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REGULATION OF CELL DEATH DURING MURINE PLACENTAL
DEVELOPMENT AND ITS DYSREGULATION DUE TO XENOBIOTIC EXPOSURE
By
Jacqueline Detmar
A thesis submitted in conformity with the requirements for the
Degree of Doctor of Philosophy
Institute of Medical Sciences
University of Toronto
© Copyright by Jacqueline Detmar 2007
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Title: Regulation of cell death during murine placental development and its dysregulation due to xenobiotic
exposure. Degree: Doctor of Philosophy Name: Jacqueline Detmar Department: Institute of Medical Science
University of Toronto, 2007
THESIS ABSTRACT:
It is well established that during human placentation, cell death is a tightly
controlled process regulating normal trophoblast turnover, differentiation and
invasion. As such, we hypothesize that cell death profiles during murine
placentation will exhibit similar features to those observed in human placenta.
Furthermore, we hypothesize that dysregulation of murine trophoblast cell death due
to polycyclic aromatic hydrocarbon (PAH) exposure will result in altered placental
cell death, having consequent deleterious effects on the fetus. Examination of
murine placental cell death over gestation revealed patterns and rates similar to
those observed in human placenta. In addition, genetic background exerted a
profound effect on cell death rates and patterns, altering developmental outcome of
both normal and PAH-induced models of placental insufficiencies. Deficiency in the
proapoptotic gene Bax resulted in intrauterine growth restriction (IUGR),
accompanied by a placental phenotype characterized by accumulation of trophoblast
giant cells and alterations in labyrinthine architecture. This gene also contributed to
embryonic lethality as in its absence, embryos were protected from PAH-induced
resorptions. In addition, we have determined that PAHs are directly responsible for
alterations in the placental vasculature, associated with deficient cell death within the
labyrinthine regiont. This event is mediated by aryl hydrocarbon receptor (AhR), as
ii
Ahf-deficient conceptuses were protected from aberrant placental cell death and
IUGR. The results of these studies indicate that murine placental death rates and
patterns parallel those observed in human placentation during normal development
and after exposure to xenobiotics such as PAHs. Thus, murine placentation
provides a useful model to investigate the molecular pathways involved in cell death
signaling during human placental development.
iil
ACKNOWLEDGEMENTS
This work could not have been achieved without the efforts of many people to
whom | will always be grateful. First and foremost, | would like to thank my
supervisors, Drs. Robert Casper and Andrea Jurisicova, from whom | not only
received academic guidance, but also moral and emotional support. Drs. S. Lee
Adamson, Isabella Caniggia and Janet Rossant deserve many thanks for their
infinite patience and careful attention to my work. | feel honoured to be indebted to
such kind and intelligent women.
Also deserving of recognition are the many members of the Casper-Brown
laboratory, for their assistance and encouragement throughout the years. A special
thank you goes to summer students, Tatiania Rabaglino, Natalie DiTomasso, Raquel
DeSouza and Roxanne Fernandes. | am very proud of their accomplishments and
am forever grateful for their help. All of my colleagues in the laboratory deserve
many thanks, not only for their technical assistance, but also for their willingness to
laugh at my bad jokes.
| wish to thank my parents, Jack and Dini Detmar, the members of my
extended family and my long-time friends for their staunch confidence in my
capabilities, for tolerating my many absences and — to me, the most important — for
opening their arms to me whenever | was in need of comfort.
Lastly, | would like to extend appreciation to the Natural Sciences and
Engineering Research Council, the Richard Venn and Carol Mitchell Fellowship, and
the Al and Hannah Perly Scholarship Fund for providing me with scholarships over
the past six years.
iv
ATTRIBUTIONS
The following people have contributed to the generation of data reported in
the present thesis:
In chapter 2, N. DiTomasso assisted with dissection and genotyping of Bax
tissues, which were originally obtained from G. Perez, University of Michigan, USA.
In chapter 3, T. Rabaglino and Y. Taniuchi assisted with genotyping Bax and
Hrk tissues. TUNEL staining and cell counts of preimplantation embryos were done
by T. Rabaglino and A. Jurisicova. Beth Acton assisted with deconvolution
microscopy of preimplantation embryos after in situ caspase-3,-7 enzyme assay and
mitochondrial membrane potential assay. AhR and Bax immunocytochemistry of
preimplantation embryos was done by A. Jurisicova, who also assisted with in vitro
treatments of blastocysts. Jaymin Oh performed dot blots of exposed embryos. The
technicians of the transgenic facility did post-treatment embryo transfers. Hrk mice
were obtained from G. Nunez and A. Benito, University of Michigan, USA. The data
presented in chapter 3 has been published in the following form: Jacqui Detmar,
Tatiana Rabaglino, Yoshinari Taniuchi, Jaymin Oh, Beth M. Acton, Adalberto Benito,
Gabriel Nunez, Andrea Jurisicova. “Embryonic loss due to polycyclic aromatic
hydrocarbon exposure is mediated by Bax.” Apoptosis 2006 11; 1413-1425.
In chapter 4, Y. Taniuchi and X. Shang assisted with genotyping AhR tissues.
M. Rennie in collaboration with John Sled and K. Whiteley did placental vasculature
casting; M. Rennie also did microCT analyses and K. Whiteley prepared casts for
SEMs and assisted with electron microscopy. Computer software programs for
microCT analyses were designed by John Sled. Ultrasound biomicroscopy was
performed by D. Qu. AhR mice were obtained from J. Tilly, Harvard University,
Boston, Massachusetts, USA.
TABLE OF CONTENTS
TABLE OF CONTENTS ........:::::ecesescesseoessssrescessccnennnsenseneessecessnneesssaeensensansesseeseness vi
CHAPTER 1: Introduction ..........ccscssssssersssssssseessssssscessssonssssensenssesesenessensenesessoseens 1
1.10 Cell death oo. eee eeccseeeeeeesneeeeeescaeeeneeeeressenaeeeeesessaneesesssneeeresses 1
1.2 Human placental development ...............cccccecccccssesseeceeseeeeesseeeesseessenes 15
1.3. Cell death in human placental pathologies................ccccccssssseeeeseseeees 18
1.4 Murine placental developMent..............sccccceceessssssssseseceesssseneesessseeeeeess 21
1.5 The mouse placenta as a model for the human placenta................... 26
1.6 The placenta and fetal programmMing...................cccccccecseseseeeceeceeeeeeneees 28
1.7 Cell death during human placental development...............c:sccccesseeeeees 29
1.8 Cell death during murine placental development..............c:cceeseseeeeees 32
1.9 Maternal exposure to cigarette smoke, polycyclic aromatic
hydrocarbons and placentation .............ccccececeeseeessesenssneseseeeeseesssseeees 40
1.10 The aryl hydrocarbon reCeptor .0......... cc ceeeeeeeseeeeeeceeeeeeeeseeeseesaseeeeeeeees 44
CHAPTER 2: Murine placental cell death exhibits an organized pattern over
gestation and placental deficiency of pro-apoptotic Bax leads to altered labyrinthine architecture and IUGR........ccsssssssssssssssessssseseeessensaconsnerssesnsessennenssszes 51
2.1 ADSEraCt ..ecccesssssssssssnecsseeeeeeceeneesesenssusensnnneeeeessensnencauneesgennecanuauenauanenssssessnssenansens 51
2.2 INTFOCUCTION...........c::eeeeceeeeeeeneeeeeseseneanennneneseesessssssonsnnanscansenensnssauseseseseessnsneneneses 52
2.3 Materials and Methods ...........:ccccsssssssnssssssssessssscscesssseessssnesssonessesnsnnnenesensenseess 55
2.3.1 Animal housing, Mating And tiSSUC COIECTION............cccccccccceeceeeseeeeeees 55
2.3.2 Terminal deoxynucleotidyl transferase dUTP nick-end labeling......... 56
2.3.3 Giant cell counts in Bax-deficient PIACENtAEC............ccccccccccceseeesneeeeeees 60
2.3.4 Immunohistochemistry and lectin histOChEMIStry ...........ccccccccccceeecees 60
2.3.5 CASPASE-3 ENZYME ASSAY .....eccceeseceeeessteceeeeeeeeetsansaeeceteenaneceesteneees 62
Vi
2.3.6 WeStern DIOTHAG 2.0... ceececeesseeceeeeseeeeeseeeecseeesecssessecnessecenecsnseaseneaes 62
2.3.7 Statistical ANALYSIS 02... ecceceeceesceeeseeceseceseeeessseessaeeesseeenseeesssusenasessaaess 64
2.4 RESUIRS........ceccsencessreessesnnnenuenesseceunesnseneeeesasenseeeeesseneaeeesessenneeseesenssneaeaenenenaaeneess 65
2.4.1. ICR and C57BI/6 conceptuses and decidua display similar numbers and patterns of TUNEL positivity at 7.5 .......cccccscsscscccesssssssceeesssssneeees 65
2.4.2 Murine placentae exhibit organized cell death patterns over gestation; however, differences in the number of TUNEL-positive cells exist Detween the twWO SUFAINS......ccccccccccccscsesssessescsesseessssnssssssnsenecseneeeeseseseess 68
2.4.3 Caspase-3 expression and localization are similar for ICR and C57BI/6 PIACONNAC. eee ee ccc ccccccccccecceeeeeeceeeeeeeeeeceesencessssecsaaaaaaaaauauaassaesseaessseesees 84
2.4.4 Bax localizes to TGCs and the labyrinth of murine placenta and Bax deficiency leads to reduced TGC death and intrauterine growth
FOSUIICTION 00. .eceeseceeceeeeseceeeeeennaeeeeeesnaneeeeetenaaeaeeeeeseccsaauasessnsaneesesesssnseees 87
2.5 DISCUSSION. ..ccccccccsssessnnsensseessssssssseesesnsenencnesecersesesnenneneseesaeeneneseessesesseeseesensesenes 100
3.1 ADStract «2.2... cceeseeeeeeeeeesseneeeeeeesaneneseanssnensssaceessoeesseneensceeessseaeneseessenseennensensagenes 110
3.2 INtrOCUCTION..........::ccceesseeeeeeenssnseeeeensnnneeeeenssenneeeseessnnaneaeeeesssneuseerasenneeerenseneoes 110
3.3 Materials and Methods ..............::ccccssseeceeesssesneeeeesssnseeesesessnsecoeseessneeneesensnssees 113
3.3.1 In vivo BaP and DMBA treatment............cccccccccessseeeesneeeesseeeesessteseens 113
3.3.2 Mating and tiSSu@ COMNOCtION ..........cccececeessesstsnneeneeeeeeeeessenssnneanenseseess 113
3.3.3 PCR GONOty Ping ............ccscccccccceeesseessssennnaceneansneeeeeeeeesssssssaaeaneneeeeess 114
3.3.4 Collection of in vivo PAH-treated preimplantation eMbry06.............. 115
3.3.5 Collection and transfer of in vittro DMBA-treated eEMbryo6..............+. 116
3.3.6 Analysis of cell number and Cell Meath .........ccccccccccceeeeeeeessttseeeeenenees 117
3.3.7 Mitochondrial membrane potential ANALYSIS...........ccccccccccssssesteeeeeees 118
3.3.8 Single EMbryO CASPASE ACTIVILY ASSAY .......cccccsssssessssscceceeccesesssnseneaes 118
3.3.9 Expression of Bax and Hrk transcripts in exposed embryos. ............ 119
3.3.10 Immunocytochemical localization of Bax And ANR.............:cccccsesseeee 120
3.3.11 Statistical ANALYSIS ........cceceeseeeessneeensaceseeensaeeeeeaeeessaeeeessaaeesnenaeess 120
Vii
3.4 RESUITS.....cccccssccscssnscecsccsesssnscesccccescccsesenensccnsssacecccnsusonsesceuesconasssuassaneesenseneceens 121
3.4.1 Effect of DMBA on murine preimplantation embryos in vitro ............ 121
3.4.2 Cellular and molecular pathways activated by DMBA...............:10000 122
3.4.3 Maternal exposure to PAHs results in decreased pregnancy and INCTEASEM FESOMPTION FALCS..........ccccccccscccececseeeeeeesssesaceececeseeeeeeensnennes 129
3.5 DISCUSSION........ccssseeeesssneressseeesseneensnneeecsaneesesseneesssannesessneneeseeeeeeseneeensensenenseeas 138
CHAPTER 4: Maternal exposure to polycyclic aromatic hydrocarbons leads to altered placental vasculature and IUGR in C57BI/6 mice, which is rescued by
ADR eFICIONCY. ............0enseassnssesesssssssececesnnecccesssesnneesensensaceaoooooosessessenssanoeouanansonnees 146
4.1 ADSI oo censnetesennenssnssnssssssenccseesneneecnecsssnanesseseeeneasooesonssaseeuseeeseeeesersconanaees 146
4.2 INTFOCUCTION.............:cecceeeesessenseseeeeeeeeeesnnssnssnsneeeeonaeceaeeusneeeesenenseanensersssereesnnes 147
4.3 Materials and Methods ............::cccsssssessessssseneesssnsseansnesonsnnsseeserssnseesesesessenenes 149
4.3.1: In vivo BaP and DMBA treatment.............cccccccccscsssececceeeeeeeeseesenennes 149
4.3.2: Mating And tisSue CONOCtION ...........cccccccceccccsecseseeceeeeeecscuanasseesesessaaaes 150
4.3.3: Vascular casting and ultraSOUNA DIOMICFOSCOPY ......cccccccccceseseeeneeeees 151
4.3.4: Terminal deoxynucleotidyl transferase dUTP nick-end labeling...... 153
4.3.5: Histological Staining...........cccccccccccccccccccceeceeceeeescsuenaneseseeeeesssseuenseanea 154
4.3.6: Immunohistochemistry and Lectin Histochemistry .............ccccceeeeees 154
4.3.7: CASPASO-3 CNZYIME ASSAY ........cccccceeecee eee e ee teeseeeeeeenenneeeeenttaneeeeeennas 155
4.3.8; WeStOr DIOTLING .2......cccceeeseennstecececeeeeeseeneeeeeeeeesnsnananeeeeeceeeesseesnenensaea 155
4.3.9: Statistical ANAlYSIS...........ccccccsceeeccceceeeceeeeeeeeeceececunnsaeeeeeseesesssensesnensea 155
4.4 RESUIES.........cccsscessssesssesssssceessnessecessnsessneeesnsessneneesnseesennenssnsnenonesnenessesssconeessnes 156
4.4.1: Maternal exposure to PAHs prior to conception leads to |UGR and altered labyrinthine vasculature in C57BYV/6 MICE... eee 156
4.4.2 Reduced umbilical vessel diameter and total fetoplacental vascular surface area and volume in d15.5 placentae from PAH-exposed dams
aneeeeeeeeeeeeeeeeeeeeeneesnseaaaeeeeeessesanaaaneaeeeeseecesesereeeeeseusecenuaneseseseseuenseenenes 159
Vill
4.4.3 Both fetal and maternal compartments of d15.5 PAH-exposed placentae exhibit altered cell death rates and changes in cell death
ITIALKOLS ooo. cece eee cceneeeeecesnneeeenenessnneeenensnsaeesensessaneesessnsaaseeeeeeseenaaaeess 164
4.4.4. AhR-deficient fetuses are protected from IUGR due to chronic maternal EOXPOSUIC 10 PAHS oo. eeccescssccseccesessnssecccssssaceeeesenssssecessssnneseesesseneneeess 182
4.5 DISCUSSION...........::::cccccesssessneseeeneeeeeneneausetessnansessasasnsanuessesnsnseneososaensoeneesesssaanes 191
CHAPTER 5: SUMMARY AND GLOBAL CONCLUSIONS ............:::sssseseserseeeees 201
-CHAPTER 6: FUTURE DIRECTIONG........sssssssssssssssssesssensessssssessseesseeenssesesense 208
1x
List of Original Publications in this Thesis
Detmar J., Rabaglino T., Taniuchi Y., Oh J., Acton B.M., Benito A., Nunez G. and
Jurisicova A. (2006) Embryonic loss due to polycyclic aromatic hydrocarbons is
mediated by Bax. Apoptosis 11: 1413-1425.
Jurisicova A., Detmar J., and Caniggia |. (2005) Molecular mechanisms of
trophoblast survival: From implantation to birth. Birth Defects Research (Part C) 75:
262-280.
LIST OF FIGURES
Figure 1.1 Schematic representation of the cell death pathway. ............cescseseceeseees 4
Figure 1.2 Schematic representations of analogous cell and tissue types between NuMAN ANd MUTLiNe PlACENtAE. .............cceeessecccceeceeeesssneneeececseeeeceeeseseceseesseessssseeeeteess 17
Figure 1.3 Schematic representations of murine placental development and the Murine placental Darricr. 20... cceseeeessseecsssneccesseccssnnesssssseeeessseeeecesensessssaueeeseneesesnnegs 22
Figure 1.4 Schematic representation of the aryl hydrocarbon receptor pathway. ... 45
Figure 2.1 Low-magnification placental section of d15.5 ICR placenta, demonstrating various regions of placenta used for histomorphometry. .................. 59
Figure 2.2 Cell death patterns in d7.5 ICR and C57BI/6 conceptuses. ...............06 66
Figure 2.3 Trophoblast giant cell death patterns in ICR and C57BL/6 placentae over
GESTATION. o.oo. eee eee eesneeeeeeeeenenaeeeeescecneeneeseeeeeeeeeseneeeeseeseesesnauseseeeceneaueeeeescnsteaeeses 70
Figure 2.4 Percentage of trophoblast giant cells containing TUNEL-positive corpses in ICR and C57BL/6 placentae over gestation. .........:ccsssscsccsssscessssseessssseessseeeesnnes 72
Figure 2.5 TUNEL patterns in ICR and C57BI/6 chorionic plate and labyrinth over GESTATION. 0... ee eeeeeensenceceeeeeeeeeeceeeeeessssenneneseeeeeessessaneeasaeasaasseceeeeaeeeeeeceseneguaeaeeas 75
Figure 2.6 TUNEL patterns in ICR and C57BI/6 junctional zone at specified tIMEPOINTS OVEF GESTATION. ..........ccccccessecceessseessssseesssseessseeeeecessseseeseueeusseeeresesseaeacsaeers 79
Figure 2.7 Maternal decidual cell death patterns in ICR and C57BL/6 placentae at specified timepoints Over Gestation. ............cccssssccccssssssceeeceeessenseteecessessneeeesessssteeeeess 82
Figure 2.8 Caspase-3 expression and activity in |CR and C57BI/6 placentae are SiMilar Over GeStatiOn. ...........: cc eeseeessceeeesessceceeeeesaeeecesenaneeaeeeeessssasseeeeeesssseeesesssnaaeess 85
Figure 2.9 Bax deficiency in murine placentae leads to decreased TGC death over GESTATION. 20... eee ceessseeeeesesensenaeeeseessesseeecessssueesesssssseseeeseceegenseeesesesssnaeeeessenetese 88
Figure 2.10 Bax deficiency in murine placentae leads to altered expression levels of placental hormones and cell death Marke’. .............cccccccseessssssseeneececeseceecececeesesenens 91
X1
Figure 2.11 Cleavage levels of active caspase-3 cellular substrates are not altered In Bax-deficient PlaCentae. ...........cecccssneccssseesssneesssseecesessseeecsssseecesssseeeesenseseseeeeesaas 93
Figure 2.12 Bax is expressed in the murine labyrinth. .............cccssssecssssesssteeesserees 96
Figure 2.13 Bax deficiency leads to abnormal labyrinthine structure and intrauterine QFOWEN FeStrICTION. .......... cece ceeeeeeeeeeeeeeeeeeeseeeeeeesssaaeeeeeeeeeeten seeeeeneeeeeteeessgaananeaeeteseeeaaaa 98
Figure 2.14 Schematic representation of cell death patterns over development in the MOUSE PIACOMMA. oo... eecceeeeseeeeeesesssssenccersceceeeeeesessussesuessseseeeeesseueesaaaasesssnssssesseseaseea 102
Figure 3.1 Exposure of murine preimplantation embryos to DMBA increases the cell death index and AhR antagonist (ANF) precedes this effect. ...............::::csceceeeeeees 123
Figure 3.2 Cell death regulatory proteins are increased in DMBA-treated murine DIASTOCYSIS. .........cccccsseseseeeccceneccseeeeecceneaceeseceesesesseessaeassseeessaaseecescsenaaseeceseesenenaeagasens 125
Figure 3.3 In vitro exposure of ICR preimplantation embryos to DMBA had no effect ON PN1 and PN21 WeiGhtS. ........ eee ee eeeceeneeeeeeeteeeeeeeeeneeeeeespeeseesseseeneneseeeeeseee 130
Figure 3.4 Chronic maternal exposure to PAHs prior to conception results in reduced cell number per blastocyst in d3.5, ICR preimplantation embryos. .......... 132
Figure 3.5 Chronic maternal exposure to PAHs prior to conception results in an increased number of resorptions and a decreased number of viable embryos, with a
greater proportion of male embryos represented in the live offspring. ................5 134
Figure 3.6 Bax-deficient, but not Hrk-deficient, embryos are rescued from resorption after chronic maternal exposure to PAHs, prior to Conception. .............ccccceeesseees 136
Figure 4.1 Maternal exposure to PAHs prior to conception leads to IUGR and altered labyrinthine architecture in C57BI/6 mice at d15.5 gestation. ................06 157
Figure 4.2 Maternal exposure to PAHs prior to conception in C57BI/6 mice results in aberrant placental microvasculature in the fetal compartment.................:::::scccceres 160
Figure 4.3 Maternal exposure to PAHs prior to conception in C57BI/6 mice results in aberrant morphology of blood spaces in maternal compartment. .............::::ccccceeee 162
Figure 4.4 Two-dimensional renderings of d15.5 fetal placental vessels from vehicle and PAH-exposed dams, after micro-computed tomography. ..............sssessssreeeeees 165
Xli
Figure 4.5 Micro-computed tomography of fetal placental casts reveals decreased
arterial surface area and umbilical vessel diameter in placenta from PAH-exposed C57BYV6 Cams. ..........cceesessecceeeeceseeeeeesaeecssateccesaeessesueecenaeseesssseeecssesesessnaeecssaeesesseas 167
Figure 4.6 Chronic exposure to PAHs prior to conception does not alter fetal heart rate, abdominal cross-sectional area, nor umbilical artery pulse velocity, as determined by ultrasound DIOMICFOSCOP)................cssssssssessssssssseeeceeeeeseesssssssesenaeee 169
Figure 4.7 Chronic exposure to PAHs prior to pregnancy leads to altered cell death patterns in d15.5 placentae of C57BI/6 Aas. ..........cccssccccssssseeessseeeesseeceessteessaees 172
Figure 4.8 Chronic exposure to PAHs prior to pregnancy leads to increased chorionic plate cell death, but TGC death is unaffected... eeccccceeseeeeee eens 174
Figure 4.9 Chronic exposure to PAHs prior to conception disrupts the expression levels of executioner caspases in d15.5 C57BI/6 placentae. ...........ccccsesseresseeeees 176
Figure 4.10 Cleavage levels of active caspase-3 cellular substrates are reduced in d15.5 PAH-exposed placentae. .0..........cccceccccseeesesceseeeeeeeeesssneeeeeescsnseeeessssaseeeeenses 178
Figure 4.11 Chronic exposure to PAHs prior to conception disrupts the balance of apoptotic and anti-apoptotic proteins in d15.5 C57BI/6 placentae. .................00 180
Figure 4.12 Chronic exposure to PAHs prior to conception up-regulated AhR expression and known target genes of AhR in C57BI/6 placentae. ...............:c0 183
Figure 4.13. Aryl hydrocarbon receptor is expressed in the fetal endothelium of the mouse placenta and AhR deficiency rescues the IUGR phenotype in dams chronically exposed to PAHs prior to CONCEPTION. ...........ccccccecessssceeeessssseceeessssneeeees 185
Figure 4.14 Maternal exposure to PAHs does not alter proliferation in d15.5 C57BI/6 placentae, as evidenced by Ki-67 immunohistochemistry.............ccccscccccessssteeeeesees 188
Figure 4.15 Maternal exposure to PAHs results in altered cell death rates in different regions of C57BI/6 placentae. ...00........eeeeesesccceeeeseseceeeeeeeeesseanereesessnseeeeesssnnseseesenes 189
Figure 4.16 Maternal exposure to PAHs prior to conception results in increased resorption rates in ICR dams and IUGR in C57BI/6 dams. ...........ccccceccessssesseereeees 196
Figure 6.1 Cell death markers in trophoblast stem cells cultured under differentiating CONCITIONS OVEF TIME. 2.0... eeeetenteeeeceeeeeeeeeeeeeeceeseaeasaeaeasessseceeeseaccesececenseeeeneeneeess 210
Xili
Figure 6.2 Polycyclic aromatic hydrocarbon treatment in ICR dams alters levels of UNK cells in early placental GECIGUA. ..........ceseeeeteeeeesesesseeeeeeeeenateserecseeeteetesnananeas 213
Figure 6.3 AhR-deficient placentae exhibit defective labyrinthine architecture and altered expression of cell death and vascular Markels. ...........sssssssesessssseeeesseeeeesses 217
XIV
2D 3D
AhR
AHRE AIF
ANF
ANOVA AP Apaf-1
Arnt
Bad
BaP Bak
Bax Bcl-2 Bcl-x,
Bcl-xs
BH3
Bid
Bik
Bmf bp:
BSA
CDI cDNA
c-FLIP CP CTB
d7.5
°C DAB DAPI
DD
DED DMBA
DMSO DNA DNase |
dNTP DRE DTT
E7.0
EndoG ECF
List of Abbreviations
two-dimensional three-dimensional aryl hydrocarbon receptor aryl hydrocarbon response element apoptosis inducing factor
a-napthoflavone analysis of variance alkaline phosphatase apoptotic protease activating factor 1
aryl hydrocarbon receptor nuclear translocator
Bcl-associated death promoter benzo(a)pyrene Bcl-1-associated killer Bcl-2-associated X protein B-cell lymphoma 2 Bcl-2-like X protein (long isoform) Bcl-2-like X protein (short isoform) Bcl-2 homology domain 3
BH interacting domain death agonist
Bcl-2-interacting killer Bcl-2-modifying factor base pairs
bovine serum albumin cell death index complementary DNA
cellular FADD-like ICE inhibitory protein chorionic plate cytotrophoblast 7.5 days post coitum
degrees Celsius diaminobenzidine
4,6-diamidino-2-phenylindole death domain death effector domain dimethylbenz(a)anthracene
dimethyl! sulfoxide deoxyribonucleic acid deoxyribonuclease | deoxynucleotide dioxin response element dithiothreitol embryonic day 7.0
endonuclease G enhanced chemifluorescence
XV
EPC
ER
FADD
Fak
FasL
FITC
GlyT Het
Hrk
IAP ICE ICM IHC
1U
JC-1
JZ kb kDa KO M
mg mL
mRNA PAH Parp-1
PBS PBST PCD PCR PECAM-1 PL-l PL-Il PN1 pNA PUMA PTEN RITC RNA sc
SDS-PAGE SE SEM
Smac SpT ST
ectoplacental cone endoplasmic reticulum
Fas-associated death domain protein focal adhesion kinase Fas ligand fluorescein isothiocyanate trophoblast glycogen cell heterozygous Harakiri inhibitor of apoptosis interleukin-converting enzyme inner cell mass immunohistochemistry
international units
5,5’,6,6’-tetrachloro-1,1’,3,3’-tetraethylbenzimidazoyl carbocyanine iodide junctional zone
kilobase pairs kilodalton
knockout molar
milligram milliliter
messenger ribonucleic acid polycyclic aromatic hydrocarbon poly (ADP-ribose) polymerase 1 phospate-buffered saline phosphate-buffered saline with 0.1% Tween 20 programmed cell death polymerase chain reaction platelet and endothelial cell adhesion molecule 1 placental lactogen | placental lactogen II post-natal day 1
para-nitroaniline p53 upregulated mediator of apoptosis phosphatase and tensin homolog
rhodamine isothiocyanate ribonucleic acid subcutaneous
sodium dodecyl sulfate polyacrylamide gel electrophoresis standard error of the mean scanning electron microscopy second mitochondrial activator of caspases spongiotrophoblast syncytiotrophoblast
XVi
TBS TBST Tdt TE TGC TUNEL WT Xiap Xist XRE Zfy1
Ug we
um
Tris-buffered saline
Tris-buffered saline with 0.1% Tween 20 terminal deoxynucleotidyl transferase trophectoderm
trophoblast giant cell terminal deoxynucleotidyl transferase dUTP nick-end labelling wildtype X-linked inhibitor of apoptosis inactive X-specific transcript xenobiotic response element
zinc finger protein 1, Y-linked
microgram microliter
micrometer micromolar
XVii
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CHAPTER 1
INTRODUCTION
Versions of sections 1.4-1.6 and 1.8 were published in Birth Defects Research (Part C), December, 2005, titled: Molecular mechanisms of trophoblast survival: From implantation to birth (Jurisicova A., Detmar J. and Caniggia I.). Reprinted with permission of Wiley-Liss, Inc., a subsidiary of John Wiley & Sons, Inc. © Wiley-Liss, 2005.
CHAPTER 1: Introduction
1.1 Cell death
Programmed cell death (PCD) is an evolutionarily conserved process that has
been documented to play a vital role during development in many diverse
multicellular organisms, including mammals, amphibians and insects. It is well
established that cell death is required for adjustment of cell number or removal of
unnecessary cellular structures such as the tadpole tail during amphibian
metamorphosis, disintegration of larval organs during insect metamorphosis,
elimination of sex specific organs such Mullerian duct in male or Wolffian duct in
females as well as formation of digits in mammals (reviewed in [1, 2]). Cell death is
also driving force behind cellular sculpturing of embryonic structures such as
creation of proamniotic cavity and formation of tubular structures [3] including neural
tube closure [4] and development of ear canal, tooth remodeling, selection of
immune cells [5, 6] as well as elimination of misplaced, injured or otherwise
dangerous cells such as ectopic primordial germ cells [7]. While this programmed
cell death is not always apoptotic in nature, as both necrotic-like and autophagic like
death have been observed to occur in some organs [8, 9], it is always tightly
regulated by conserved molecular pathways, guarding the decision and execution of
cell death machinery [10, 11].
Bcl-2 family members
Proteins of the Bcl-2 (B-cell lymphoma 2) family are crucial regulators of the
cell death pathway (reviewed in [12, 13]). This family is composed of multi-domain,
anti-apoptotic (Bcl-2, Bcl-X,_, Bcl-w, Mcl-1) proteins which associate with several
cellular organelles, including the outer membrane of the mitochondria, the
endoplasmic reticulum (ER) or nuclear membranes and contain four characteristic,
homologous regions, called Bcl-2 homology domains (BH1-4) [14]. Their
counterparts are the multi-domain, pro-apoptotic (Bax, Bak, Mtd, Bcl-xs) proteins
that also bear BH domains — typically three or four — and act in an antagonistic
fashion to the pro-survival molecules. Additional family members include the BH3-
only proteins, which are pro-apoptotic proteins containing only the BH3 domain
(Bad, Bik, Blk, Bim, Bid, Hrk/DP5, Noxa, PUMA). The BH-3 only proteins act as
sentinels, charged with activating the cell death pathway in response to a variety of
different death stimuli. The BH3 domain is critical for engaging the anti-apoptotic
Bcl-2 proteins and rendering them inactive, thus triggering the cell death cascade
[15]. The mitochondria are the primary sites of actions of the Bcl-2 family members,
with functionally opposing proteins heterodimerizing via the BH domains. These
actions are mediated by the interactions of the BH3 a-helix on the pro-apoptotic
protein cleft formed by the a-helices of the BH1, BH2 and BH3 regions of the anti-
apoptotic proteins [16]. Therefore, both multimeric and BH3-only family members
can induce cell death by binding to pro-survival proteins such as Bel-2 and Bcl-x;
however, the BH3-only proteins cannot kill in the absence of their multi-domain
cousins, such as Bax and Bak [17].
The extrinsic cell death pathway
Death receptors and their cognate ligands belong to the tumour necrosis
factor (TNF) gene superfamily. The best characterized of these are the Fas (CD95,
Apo-1)/FasL (Fas ligand; CD95L, Apo-1L) and the TNF/TNF receptor pathways.
While the molecular mechanisms involving death receptor ligation have largely been
elucidated through studies involving cells of the immune system [18], Fas and TNFR
are expressed in a number of different cell types, including trophoblasts [19-21].
Death receptor ligands can exist in soluble form, exemplified by TNF-a or in
membrane-bound form, such as FasL or TNF-related apoptosis-inducing ligand
(TRAIL). Additionally, FasL has been shown to exist in soluble form (sFasL),
generated by proteolytic cleavage of membrane-bound FasL by matrix
metalloproteinases [22, 23], or sequestered in secretory vesicles and released into
the circulation or extracellular space [24]. Membrane-bound death receptor ligands
are largely involved in immune cell homeostasis [18] and maintaining sites of
immune privilege [21, 25]; however, the exact role of secreted ligands is
controversial, as they have been shown to have either cytoprotective or cytotoxic
capacities [24, 26].
External death cues are transmitted through death receptors located at the
cell membrane, such as the Fas receptor (CD95, Apo-1), the tumour necrosis factor
receptor (TNFR) or death receptors 3-6 (DR3-6). Ligand-bound receptors require a
set of signaling proteins bearing a distinct set of modular domains to facilitate
homotypic interactions (Figure 1.1). The Fas molecules associate to form a trimeric
Death Signal
(FasL; TNF, etc.)
Death Adaptor ae
<< Protein Te : “ (FADD, TRADD) ° ON DW
a, Death ae Si,
Receptor. v8 Procaspase-8/10
Active
caspase-8/10
@ ATP “**-@ Smac _
&
\ Be
%, @ Apat-t _-” Cytochrome ¢ & i \ ae “en
© . J Posse me Active y mG
Procaspase-3 ¢ caspase-3. @ vie ay
mea ar
pe
ON APOPTOSOME &
Procaspasé-3 lL .
Procaspase-6 ¢ | |
: . Cleavage of cytoplasmic Procaspasé-7 Active effector , and nuclear proteins Chromatin
a caspases condensation DNA YS CELL fragmentation
DEATH Nucleus
Figure 1.1 Schematic representation of the cell death pathway.
complex, with each receptor bearing a cytoplasmic tail containing the death domain
(DD), which will ultimately trigger the formation of the death-inducing signalling
complex (DISC; [27]). A cytoplasmic adaptor molecule, Fas-associated death
domain protein (FADD), also bears a DD at its C-terminus and homotypically
associates with the DD of the Fas receptor [27]. At the N-terminus of the FADD
protein is a death effector domain (DED) which binds with the DED of initiator
caspases, such as procaspase-8 or -10, through homophilic interactions. The
sequestration and clustering of these proenzymes allows autoproteolytic processing,
thereby forming active caspases [18, 27]. Inhibition of death receptor-induced
activation can be effected at this point, by cellular FADD-like interleukin-converting
enzyme inhibitory protein (c-FLIP). This protein bears two DED domains and a
caspase-like domain similar to caspase-8 but lacks proteolytic capability, thus
competitively blocking autocatalysis of the procaspases [28, 29]. Once the initiator
caspases have been activated, they cleave downstream effector pro-caspases
(caspase-3, -6, -7), producing active proteases with a variety of specific cellular
targets [30], resulting in the morphological and biochemical hallmarks of cell death
[31]. The extrinsinc death pathway can also lead to activation of mitochondrially-
mediated cell death, as caspase-8 can cleave the pro-apoptotic, BH3-only family
member, Bid, forming truncated Bid (tBid), which translocates to the mitochondria,
activating Bax and releasing cytochrome c [32, 33].
The intrinsic cell death pathway
The intrinsic cell death pathway is triggered by cellular stress signals such as
DNA damage, oxidative stress, toxin exposure or growth factor deprivation. The
common link in achieving cellular demise via these triggers is the engagement of cell
organelles, particularly the mitochondria (Figure 1.1). Proapoptotic Bcl-2 family
members such as Bax and Bak remain cytosolic until activation by apoptotic signals.
Upon stimulation, these proteins translocate to the mitochondria and form
membrane-spanning, oligomeric pores, in an as-yet, unresolved mechanism [34],
facilitating the release of several apoptotic factors, including cytochrome c,
Smac/Diablo [85, 36], endonuclease G (EndoG) [37, 38], apoptosis-inducing factor
(AIF) [39, 40] and Omi/HtrA2 [41]. In the presence of ATP/dATP, released
cytochrome c and apoptotic protease activating factor-1 (Apaf-1) recruit initiator
caspase-9, which undergoes autoproteolytic cleavage when bound to Apaf-1,
forming the oligomeric complex, the apoptosome [42]. This macromolecular
complex can then facilitate activation of downstream effector caspases, including
caspase-3, -6 and -7, which destroy or inactivate specific cellular substrates,
resulting in the demise of the cell.
Triggering cell death via the mitochondrial pathway is reliant upon several
Bcl-2 family members, including membrane-associated proteins such as Bax, which
mediate the release of apoptogenic factors from the mitochondria.
Bax — a multidomain, pro-apoptotic Bcl-2 family member
In healthy cells, Bax is a cytosolic, monomeric protein that functions in cell
death through the mitochondrial pathway [43, 44] recent evidence suggest that this
protein can also localize to the ER, functioning in an unknown role [45]. Both Bax
and Bak are widely distributed, with expression reported in many cell and tissue
types, functionally substituting for each other [45]. During apoptosis, Bax changes
conformation and integrates into the outer mitochondrial membrane and
oligomerizes, forming the mitochondrial apoptosis-induced channel (MAC) [46]. This
permeabilizes the mitochondrial membrane — via controversial mechanisms [47] —
allowing the efflux of apoptogenic proteins into the cytoplasm [48]. Recent studies
using Hela cell lines have demonstrated that Bax and Bak are functionally redundant
in the formation of the MAC complex [46].
Targetted knockout of Bax in mice revealed a series of defects including
lymphocyte hyperplasia, accumulation of neurons, abnormal ovarian follicle
morphology and accumulation of germ cells in the testes that renders Bax-deficient
males infertile [49]. Furthermore, while Bak knockout mice were developmentally
normal and fertile, Bax/Bak double knockouts typically died in the perinatal period
and exhibited persistence of the interdigital webbing, imperforate vaginal canal and
accumulation of cells in both the hematopoietic and nervous systems [50]. The
results of this study revealed that Bax and Bak have overlapping functions with
respect to apoptosis. These proteins execute crucial cell death functions during
mammalian development and tissue homeostasis, regulating the release of
apoptogenic factors from the mitochondria.
Mitochondrial mediators of apoptosis
While members of the Bcl-2 family control the mitochondrial response to
death signals, various factors released from this organelle have a critical function in
the apoptotic process (Figure 1.1) [51]. The first identified mitochondrially-derived
apoptotic factor was cytochrome c, which, until then, had been a known player in the
oxidative phosphorylation pathway, having a role as an electron shuttle protein [52].
The release of cytochrome c contributes to the formation of the apoptosome and
subsequent cleavage of downstream effector caspases. It is currently believed that
only a portion of cytochrome cis released, functioning in the apoptotic pathway and
the fraction of cytochrome c remaining in the mitochondria will continue to sustain
ATP production [53, 54]. Over time, the progressive damage to the mitochondria
becomes irreversible, ensuring cell death. The primary role of second mitochondria-
derived activator of caspase (Smac) in this pathway is to act as a molecular brake,
antagonizing the inhibitors of apoptosis proteins (IAPs), cytosolic proteins which
block the activity of various caspases, including caspase-3, -6 and -9. The
apoptosome complex was shown to contain the X-linked IAP (Xiap), which binds and
sequesters active caspase-3 and -9, thus blocking the proteolytic cascade [55]. If
the apoptotic stimulus is persistent or great in magnitude, the [AP-binding
capabilities of mitochondrially-derived proteins such as Smac, will competitively bind
cytoprotective proteins such as Xiap.
The three remaining mitochondrially-sequestered, death-inducing proteins
have been studied only in a limited context. Omi/HtrA2 is a protein with a dual
nature, as it can mediate caspase-dependent death through its ability to inhibit IAPs,
in addition to its function as a serine protease [41]. Overexpression of this protein
revealed the essential function of the catalytic domain for inducing caspase-
independent death [56]. Endonuclease G is another mitochondrially-derived protein,
shown to be localized to the nucleus under the influence of certain death stimuli, in
the context of both caspase-dependent and independent death [37]. While EndoG
has been implicated in the degradation of DNA [88], the exact role and relevance of
this molecule is uncertain. Lastly, AIF is a flavoprotein that normally executes an
oxido-reductase function in healthy cells [57]. In addition to this role, AIF is released
from the mitochondria during apoptosis and translocates to the nucleus to act as
mediator of chromatin condensation and DNA fragmentation (greater than 50 kb)
[39, 40]. The mitochondrial mediators of apoptosis are crucial for cell viability, as
cytochrome c [58], AIF [59] and Omi/HtrA2 [60] knockout mouse models exhibit
either embryonic or postnatal lethality; however, some redundancy in function
amongst these molecules and other cellular proteins does appear to exist, since
Smac- and EndoG-deficient mice are viable and have limited phenotypes linked to
the apoptotic mechanism [61, 62].
Caspases
Caspases are cysteine-dependent aspartate-directed proteases that are
present as inactive zymogens and are cleaved to an active form either
autocatalytically or by up-stream caspases. In Caenorhabditis elegans, CED-3 was
identified as a protease critically involved in the developmental cell death process.
The first mammalian caspase was originally discovered as a cytokine processing
10
enzyme and was known as interleukin-1-B-converting enzyme (ICE); since then,
fourteen different homologues have been identified [63]. Based on their prodomain
length and composition, caspases can be subdivided into upstream initiator
caspases (such as caspase-2, -8, -9 and -10) and short domain effector caspases
(caspase-3, -6 and -7). Initiator caspases possess long prodomains containing
either a DED or a caspase activation and recruitment domain (CARD), or both.
These regions facilitate interactions with adaptor molecules and promote the
process of autoproteolysis, a characteristic unique to the initiator caspases. Upon
activation, the initiator caspases cleave downstream effector caspases which act as
executioners of the cell death pathway. Active caspases are capable of cleaving
various intracellular proteins, including, but not limited to, structural elements of the
cytoplasm and nucleus, signaling molecules and proteins involved in DNA damage
repair. This leads to the disruption of survival pathways and the disassembly of
important architectural components of the cell, contributing to the morphological and
biochemical changes that characterize apoptotic cell death [30, 31].
One of the downstream targets of active caspase-3 is poly(ADP-ribose)
polymerase-1 (Parp-1), a crucial enzyme capable of binding DNA and mediating
base-excision repair, thus maintaining genomic integrity [64, 65]. Parp-1 responds
immediately to cellular stresses (radiation, ischemia, genotoxins) that result in DNA
damage, in a process that is energetically expensive. Therefore, high levels of DNA
repair lead to depletion of cellular energy stores by Parp-1, resulting in necrosis.
Thus, it is believed that the cell’s response to substantial genomic damage is to
induce apoptosis, thereby protecting neighbouring cells from the harmful,
11
proinflammatory effects of necrotic cell death [65]. A consequence of triggering the
cell death cascade is the cleavage of Parp-1 into canonical 24-kDa and 89-kDa
fragments [66, 67]. As such, the cleavage profile of Parp-1 afer Western blotting has
provided an end-point assay for the detection of cell death signaling within a
eukaryotic system [68].
There are a number of different caspases, some of which are only
peripherally involved in the regulation of cell death. The primary targets of such
caspases are proteins required for other non-apoptotic cellular responses, such as
cytokine maturation, cellular differentiation and cell cycle progression (reviewed by
[69, 70]. Furthermore, different caspase family members appear to have distinct
subcellular localization and cleave different subsets of proteins, dependent upon the
apoptotic trigger or cell type [71]. Investigations of cell death pathways in several
physiological models revealed that cells lacking certain kinds of caspases will
compensate by upregulating another caspase with similar substrate specificity [72].
Nonetheless, physiological animal studies have revealed requirements of certain
caspases in distinct cell types and along different stages of development [69].
Alternate modes of cell death
Recent evidence suggests a greater diversity in the cell death programme, as
an apoptotic-like death can occur without the activation of effector caspases. Signals
originating from established apoptosis-related factors such as death receptors,
caspases and certain Bcl-2 family members, may result in morphological and
biochemical features consistent with non-classical cell death. In addition to
12
apoptosis (Type | death), other cell death pathways include necrosis, autophagy
(Type II death), mitotic catastrophe, and senescence, which has been described as
a “living cell death” [73].
Autophagy is a non-necrotic, caspase-independent death, hallmarked by cell
membrane blebbing, partial chromatin condensation, autophagic vesicles within the
cytoplasm and increased lysosomal activity [74]. The genetic basis of autophagy is
conserved across evolution, with homologous genes identified in organisms from
yeast to humans [75]. Two types of autophagy exist, microautophagy and
macroautophagy. Microautophagy is characterized by engulfment of cellular
materials directly adjacent to the lysosomal membrane, whereas macroautophagy
consists of surrounding portions of the cytosol with double-membrane vesicles,
sequestering the contents to be degraded from the rest of the cytoplasm. Fusion of
the vesicle with lysosomes - forming an autophagosome — allows the cargo to be
degraded in a closed system, thereby protecting the cell from potentially cytotoxic
constituents [11]. The autophagic process allows recycling of old proteins and
organelles, while also providing the cells with basic building blocks for renewing
cellular machinery and structure. Triggering of the autophagic mechanism occurs
during cellular response to nutrient starvation, growth factor withdrawal, high
temperatures, hypoxia and invasion of pathogens [11, 74, 75]. However, autophagy
has also been reported to have requisite functions during development, allowing
dauer development in C. elegans [76], remodeling of the salivary glands in
Drosophila [9] and regression of the Mullerian ducts in mammals [77]. Dysregulation
of the autophagic process can result in a number of disease states, including cancer
13
[78] and the degenerative disorders, Huntington’s, Alzheimer’s and Parkinson’s
diseases [79]. Lastly, a number of Bcl-2 family members have been implicated as
having a role in autophagic cell death, including Bax, Bak, Bcl-2 and Bcl-x, [74].
Necrosis, in contrast to both apoptosis and autophagy, is not a self-contained,
regulated process, resulting in traumatic cell destruction, followed by the release of
the intracellular contents in the immediate vicinity [80]. Induction of necrosis is
typically triggered by events that have a radical and immediate effect on the cell
metabolism and machinery; these types of exposures often affect large numbers of
cells simultaneously. Examples are respiratory poisons, irradiation, physical
disruption of cellular membranes caused by altered extracellular osmolarity, extreme
pH, extreme temperatures and physical trauma [81]. In the presence of such
stressors, the cell will have difficulty producing ATP, thereby compromising ion flux
and water balance. This creates leaks in the cell membrane, causing the cell to
typically gain water and sodium ions and leading to cellular swelling. In turn, calcium
ions and other cellular constituents can leak out of the cell, causing damage to the
surrounding tissue. At this point, cellular metabolism stops and the DNA begins to
degrade in a completely nonspecific fashion. Internal membranes from organelles
such as lysosomes and peroxisomes can also be compromised, releasing their
contents into the cell itself and eventually, into the neighbouring environment [82].
Necrosis is generally deemed to be a passive process; however, there appears to be
a modicum of regulation involved and while some players of the necrotic pathway
have been identified, the underlying signaling pathways remain enigmatic [73, 82].
Finally, a number of studies have recently reported the presence of cell death with
14
necrotic features under normal physiologic conditions, as seen during renewal of
enterocytes in the small intestine [83] and during follicular maturation in the ovary
[84] . Moreover, necrotic cell death has been observed to compensate for the lack
of apoptotic proteins in mice deficient for classical cell death genes [8, 85].
Apoptosis-related molecules have functions outside of cell death
Recent evidence suggests that proteins having a well-established role in cell
death pathways have alternate functions in other cellular processes such as
proliferation, differentiation and survival. In fact, the first identified mammalian
caspase, caspase-1, was originally described by two separate groups [86, 87] as a
protease involved in cytokine maturation and was given the moniker, interleukin-
converting enzyme (ICE). Upon the cloning of the C. elegans cell death gene, ced-
3, ICE was found to be homologous in sequence and structure, and mammalian
ICE-like proteases were later discovered to have key roles in the apoptotic pathway
[88]. Both initiator and effector caspases have been linked to having roles outside of
cell death. Caspase-8 has been linked to not only lymphocyte proliferation, but has
also been shown to serve a role in trophoblast and macrophage differentiation in
both humans [89, 90] and mice [91, 92]. Similar functions have been indicated for
caspase-3, with reported involvement in B-lymphocyte [93] and neuronal [94]
proliferation and also in erythroblast [90], myoblast [95] and osteoblast [96]
differentiation. Thus far, it appears that caspases mediate their effects through
cleavage of various cellular substrates, and it is speculated that whether the
15
outcome is apoptotic or non-apoptotic depends on the extent of caspase activation
[97].
In addition to caspases, members of the Bcl-2 family have also been
implicated in having roles outside of cell death. Brady et al. [98] reported that mice
transgenic for Bax overexpression in the T-cell lineage results in an increased
number of cycling thymocytes. Furthermore, upon IL-2-induced stimulation, these T-
cells were capable of entering the S phase faster than control cells. More recently, it
was shown that mice deficient in p53 and transgenic for constitutively-expressed, T-
cell-specific Bax, exhibited a greater incidence of T-cell lymphomas compared with
p53-deficient mice [99]. In addition to regulating cell cycle events, both Bax and
Bak were demonstrated to be required in healthy cells for normal fusion and fission
of mitochondria [100]. Interestingly, while pro-apoptotic Bcl-2 family members
appear to accelerate entry into the cycle, anti-apoptotic members seem to have an
anti-proliferative effect. Transgenic mice over-expressing Bcl-2 in cells of B- and T-
cell lineage exhibited decreased lymphocyte turnover and slower entry into the cell
cycle after exposure to mitogens [101, 102]. Moreover, similar anti-proliferative
effects were observed in anti-apoptotic members, such as Bcl-xL, Mcl-1 and Bcl-2
(reviewed in [103}).
1.2 Human placental development
The placenta is a life-sustaining organ, which mediates the physiological
exchange of oxygen, nutrients and waste between mother and fetus. During human
placentation, highly proliferative cytotrophoblast (CTB) cells reside in chorionic villi of
16
two types, floating and anchoring villi. Floating villi are bathed in maternal blood and
allow gas and nutrient exchange for the developing embryo; the CTB of such villi
proliferate extensively during the first trimester and differentiate by fusing to form the
multinucleate syncytiotrophoblast (ST) layer (Figure 1.2). This layer is subject to
continuous renewal, whereby aged nuclei, together with cytoplasm, are released into
the maternal circulation as syncytial knots, to be replaced by the fusion of new CTB
cells [104, 105]. Cytotrophoblast cells in anchoring villi have two fates: either to fuse
and form the ST or, at selected sites, break through the basement membrane and
form columns of extravillous trophoblast cells (EVT). These columns physically
connect the embryo to the uterine wall and provide individual EVT cells that migrate
and invade the maternal spiral arteries of the placental bed [106]. This results in the
conversion of narrow arteries into distended uteroplacental arteries, which increases
blood flow to the placenta, providing oxygen and nutrients to the growing fetus.
Dysregulation of the cell death programme has been implicated in a number
of human gestational diseases, including preeclampsia and intrauterine growth
restriction (IUGR). Investigations into these pathologies have helped to elucidate
the cellular mechanisms of trophoblast cell death in both normal and diseased
states.
17
Human Placenta Mouse Placenta
Syncytiotrophoblast a Labyrinthine region with proliferative
Proliferative cytotrophoblast cells stem cells
Proximal extravillous trophoblast cells [|] Junctional zone with spongiotrophoblast
Distal extravillous trophoblast cells a Trophoblast giant cells
Syncytial knots @8 Trophoblast glycogen cells
Maternal decidua [|] Maternal decidua
td Maternal spiral artery ? Maiernal spiral artery
Figure 1.2 Schematic representations of analogous cell and tissue types between human and murine placentae.
18
1.3. Cell death in human placental pathologies
Preeclampsia
The majority of studies have focussed on pre-eclampsia, a placental disorder
complicating 5-7% of of pregnancies and is a major cause of maternal and perinatal
morbidity and mortality. This disease is associated with excessive shedding and
deportation of placental debris into the maternal circulation, due to unscheduled ST
cell death [107-109]. Syncytiotrophoblast renewal is facilitated by a balance of CTB
proliferation and syncytial knot release. It has been postulated that the elevated
levels of CTB proliferation observed in preeclamptic villi [110] perturb this balance,
thus forcing the ST to maintain integrity by increasing syncytial knot shedding [111].
This is believed to overwhelm the apoptotic machinery in ST cells, leading to a
truncated form of apoptosis, followed by necrosis, in a process termed “aponecrosis”
[112]. The release of non-apoptotic placental debris into the maternal circulation
results in the wide-spread, intravascular inflammatory responses noted in
preeclamptic women [107, 113]. Moreover, the Fas/FasL pathway has been
implicated in the pathophysiology of preeclampsia, as increased levels of Fas and
decreased levels of FasL have been detected in villous trophoblast [114]. Lastly,
sera from preeclamptic women have been shown to induce trophoblast cell death via
Fas-mediated sensitization [20].
Trophoblast differentiation and invasion are also impaired in preeclampsia,
leading to insufficient remodelling of the maternal spiral arteries, which retain their
vasocontrictive abilities, thus reducing placental perfusion [115-117]. In addition,
19
elevated apoptotic indices have been observed in EVT of preeclamptic placental
beds [118, 119], contributing to the arterial defects. Inadequate placental perfusion
results in a number of deleterious consequences, including placental oxidative
stress, hypoxia, ischemia/reperfusion injuries and infarcts [120, 121]. Thus, a large
number of symptoms of preeclampsia are directly and indirectly associated with
aberrations in the placental cell death programme.
Intrauterine growth restriction
Optimal embryonic and fetal growth depend upon the interaction of genetic
and environmental factors, including embryonic and maternal genetic and hormonal
profiles, adequate nutrient and oxygen supply and the appropriate development and
regulation of the maternal-placental-fetal unit. Approximately 7-9% of live infants
exhibit birth weights below the 10" percentile [122], a diagnostic feature of IUGR.
Intrauterine growth restriction is considered to be a pathological reduction in
expected fetal growth, due to intrauterine factors. This is distinct from babies that
are small for gestational age, which is based on standard values of infant weight and
is not reflective of fetal and neonatal growth dynamics [123]. There are a number of
established causes for IUGR including preeclampsia, fetal infection, malnutrition,
placental damage and exposure to cigarette smoke [123]. IUGR is further classified
as either “symmetric” or “asymmetric”. Symmetric IUGR is a proportional decrease
in length, weight and head size, while in asymmetric IUGR, the length and weight
are decreased, but there is a head sparing effect such that fetal head circumference
is appropriate for gestational age [124]. Determination of intrauterine growth is
20
assessed by the following ultrasonographic measurements: biparietal diameter,
abdominal circumference, femur length and crown-rump length [125]. While IUGR is
linked to increased rates of perinatal morbidity and mortality, it has also been
associated with the onset of childhood and adulthood cardiovascular and metabolic
diseases [123].
Placental insufficiency is a significant contributor to |UGR [123]. Known
placental pathologies of IUGR include decreased placental growth, chronic villitis,
increased fibrin deposition, umbilical cord anomalies, infarct, CTB hyperplasia and
basement membrane thickening [126-128]. In addition, overall size and surface
area are decreased in IUGR placentae, and they exhibit smaller terminal villi and
abnormal villous vasculature [129, 130]. Reduction in placental size has been
attributed to increased rates of cell death [131-134]. A number of different placental
cell subtypes appear to be affected, with unscheduled death seen in chorionic
trophoblast [135], villous stroma and trophoblast [132] and ST [126]. On the
contrary, ultrastructural studies of IUGR placentae have revealed no difference in
cell death rates [128]. Additionally, while serum from preeclamptic women
demonstrated higher levels of ST microparticle shedding, this was not observed in
women with normotensive IUGR [109]. Some of the discrepancies in apoptotic rates
have been attributed to differences in experimental technique and tissue sampling.
Moreover, the underlying molecular mechanisms involved in the pathogenesis of
IUGR are largely unresolved and might confound trophoblast cell death analyses.
21
1.4 Murine placental development
The murine embryo at implantation (d4.5) has a simple trophectoderm
surrounding the blastocyst, which will eventually give rise to all trophoblast cells in
the placenta (reviewed in [136, 137]). Trophoblast stem (TS) cells emerge from a
population of cells known as the polar trophectoderm, which overlies the inner cell
mass of the embryo. Contact with the inner cell mass causes the TS cells to
proliferate, in a process that is mediated by the growth factor, fibroblast growth factor
4 (FGF-4) [136]. Trophoblast stem cells are multi-potent, can proliferate in culture
for many generations [138] and can differentiate both in vitro and in vivo, into a
number of different trophoblast cell subtypes [139]. At day 6 of mouse development,
two diploid populations of trophoblast derivatives are established: the extra-
embryonic ectoderm and the ectoplacental cone (EPC; see Figure 1.3a).
The labyrinthine region
Between days 7.5-9.5 the placenta undergoes major morphological
remodeling, resulting in the formation of three distinct cellular regions, each with
unique morphology and function (reviewed in [136, 137]). Chorioallantoic (CA)
attachment transpires at approximately d8.5, a process whereby the allantois
attaches and interdigitates with the chorion [142]. Thereafter, nascent villous
branches become evident and are lined by very thin and elongated trophoblast cells
[142]. Further branching establishes a network of villi perfused with fetal blood
22
Figure 1.3 Schematic representations of murine placental development and
the murine placental barrier. A. Depicts the different regions or cell types with the
mouse placenta from early implantation to midgestation to late gestation. B.
Depicts the murine placental barrier, or interhemal distance. Panel B was based on
transmission electron micrographs published in Georgiades et al., 2002 [140] and
Coan et al., 2005 [141].
["] . maternal decidua
[-].. junctional zone
labyrinth
[| chorionic plate
GP trophoblast giant cells
@3 trophoblast glycogen cells
? maternal spiral artery
fetal trophoblast layer |
"| syncytiotrophoblast layer II
syncytiotrophoblast layer III
fetal capillary endothelium
23
d7.5
Uterine cavity
———__— Secondary TGC i —————-— Ectoplacental cone
Allantois
Primary. TGC
Proximal and distal endoderm
d10.5
Fetal capillary lumen
Figure 1.3
24
embedded in numerous small canals perfused by maternal blood. This region is
collectively referred to as the labyrinth (see Figure 1.3a) and is the site of fetal-
maternal exchange. During this process, the chorionic trophoblasts differentiate,
giving rise to several different cell types [143], that form the interhemal placental
barrier (Figure 1.3b). This barrier is comprised of four layers of cells that separate
the fetal and maternal circulatory systems. Lining the maternal blood spaces and
forming the first layer of the placental barrier are large, mononucleate, post-mitotic
cells, now considered to be a subtype of trophoblast giant cell (TGC), with a role in
hormone production [143]. Lying underneath, are two layers of ST cells, known as
syncytiotrophoblast layer II (proximal to maternal blood spaces) and
syncytiotrophoblast layer III (distal to maternal blood spaces). Formation of the ST
layers is a result of cell-cell fusion, which is mediated in part, by the apoptotic
pathway [104, 144]. At the time of CA attachment, the blood vessels and
mesenchyme — originating from the allantoic mesoderm — begin appearing within the
labyrinth [143] . The fetal endothelium is the fourth layer of the placental barrier.
The labyrinth of the mouse placenta is responsible for gas and nutrient exchange.
Studies involving gene knockout mice have underscored the crucial role the labyrinth
plays in maintaining viability of the fetus [145, 146].
The junctional zone
The junctional zone lies between the labyrinth and the TGC border and is
composed of spongiotrophoblast (SpT) and glycogen cells (GlyT; Figure 1.3a).
25
Spongiotrophoblast cells likely arise from the EPC, based on their strong similarities
in gene expression [137]. The SpT provides structure and support to the labyrinth
and consists of variable-sized, hormone-producing cells that appear to have limited
proliferative capabilities [147]. While the precise function of the SpT remains
enigmatic, targeted gene knockout studies have shown that disrupting this layer can
lead to embryonic lethality [148, 149]. Large, maternal blood channels pass through
the SpT and are lined by fetal trophoblast cells [147, 150], forming the maternal
blood spaces. These canals undergo extensive branching within the labyrinthine
layer, forming the maternal blood spaces, which are lined by trophoblast cells, as
described earlier. Although not completely established, it appears likely that SpT
cells can differentiate into GlyT [140, 143], which begin appearing at approximately
d12.5 [150]. These cells have a characteristic morphology, containing glycogen-rich
vacuoles and appear clustered together, forming islets within the junctional zone.
Later in gestation, GlyT invade the maternal decidua in an interstitial fashion, where
they enter a lytic phase at approximately d17.5, possibly supplying the surrounding
cells with an energy source for impending parturition [151].
Trophoblast giant cells
The trophectoderm of the blastocyst that is not in direct contact with the inner
cell mass is called the mural trophectoderm. From this population of cells arises the
primary TGCs (Figure 1.3a), which exit the cell cycle and undergo
endoreduplication, a process involving DNA replication without intervening karyo-
and cytokinesis [152, 153]. These cells then migrate to the antimesometrial pole of
26
the embryo and surround the future parietal yolk sac [143]. Secondary TGCs arise
from the cells of the EPC and later, from cells of the SpT [154]. These celis are
morphologically distinct, undergoing many rounds of endoreduplication, forming
large, polyploid nuclei. A clear border of secondary TGCs is evident in murine
placenta, separating the fetal junctional zone and the maternal decidua (Figure
1.3a). While not all the functions of TGCs have been fully elucidated, these cells
clearly have a role in implantation and invasion [137]. In addition, secondary TGCs
have been shown to produce luteotropic and lactogenic hormones, as well as
angiogenic factors [147], promoting maternal physiological adaptations to
pregnancy, parturition and future nourishment of the neonate [155]. While the
secondary TGCs comprising the giant cell border migrate only short distances, a
specialized subtype known as endovascular TGCs (EndoTs), are capable of
invasion and remodeling maternal spiral arteries [147]. These cells are
morphologically distinct, appearing smailer and more spindle-like in shape [156].
Moreover, EndoTs have a different gene expression profile compared with that seen
in TGCs comprising the giant cell border [143], supporting the idea that these cells
are a specialized subtype.
1.5. The mouse placenta as a model for the human placenta
Recent comparative studies between mouse and human placentae [140, 157]
have revealed striking similarities in cellular mechanisms and tissue framework,
providing justification for using the mouse placenta as an animal model for the
27
human placenta. The labyrinthine region of the mouse placenta is the site of
maternal-fetal exchange and exhibits a similar mechanism of syncytialization to
properly maintain the placental barrier [142]; thus, the labyrinth bears a similarity to
floating chorionic villi in humans (Figure 1.2). The junctional zone is considered
analogous to human column CTB cells, based on: the expression of several gene
markers; its role in structural support; its spatial distribution; and, its ability to give
rise to terminally differentiated GlyT cells [157, 158]. Trophoblast glycogen cells and
TGCs are capable of invading and directly contacting the maternal decidua and
therefore, are considered to be the murine equivalent of human EVT cells [159]. To
further support the use of the mouse as a model organism for human placentation,
recent studies have reported that during murine placentation, the maternal spiral
arteries are remodeled by specialized, invasive trophoblast cells [147, 150]. This is
identical to those events occurring during human placentation, where the spiral
arteries of the placental bed are invaded by EVT cells.
There are, of course, a number of important differences between the mouse
and human placenta. The majority of mammals, including non-human primates
exhibit superficial implantation and limited invasion of trophoblast cells into the
decidua, compared to that seen during human placentation [157]. Rodent
pregnancies are relatively brief and give birth to a litter of young that are
comparatively immature to human neonates. Additionally, the placental barrier
includes three trophoblast layers in the mouse, whereas in the human placenta, this
structure is comprised of a single layer of trophoblast and a discontinuous second
layer of CTB [140]. Nonetheless, the presence of homologous cell types and cellular
28
behaviours highlight the use of the mouse as a suitable model for the study of
normal placentation. Such a model is highly attractive, as it allows for genetic
manipulation and induction of various pathological conditions.
1.6 The placenta and fetal programming
In the last decade, substantial evidence has supported the idea that a
compromised in utero environment can influence health during postnatal life. Barker
[160] introduced the concept of fetal programming (heretofore referred to as the
Barker Hypothesis), which proposes that a number of organ structures and functions
undergo programming during embryonic and fetal life. This developmental
programming determines the physiologic and metabolic set points, which will
ultimately cue responses to the environment in the adult. Adverse in utero
conditions, such as placental insufficiency, inadequate maternal nutrition, and
altered maternal stress hormone profiles lead to developmental adaptations by the
embryo/fetus that readjust these set points (reviewed by [161, 162]). These
adaptive measures ostensibly have short-term benefits to the embryo and fetus, but
these changes to the genetically-determined body plan may confer a discordant
physiology on the adult, leading to increased risk of disease. It has been repeatedly
shown in human populations that IUGR fetuses resulting from placental insufficiency
are at increased risk for adverse short- and long-term outcomes such as
hypertension, obesity and type II diabetes, that can extend into adult life [160, 163-
165]. There is a rapidly-growing body of evidence suggesting that the placenta is
involved in fetal programming (reviewed by [166, 167]), with particular emphasis on
29
the impact of placental insufficiency on fetal cardiac development [168], fetal neural
development [169-171] and fetal endocrinology [172]. Proper establishment of the
placenta at these times allows the fetus to grow and attain its developmental
potential in the third trimester, in preparation for postnatal life. Investigations into
how normal placental cell death assists in shaping placental architecture and
function will provide us with information to better understand how aberrant or
insufficient cell death in this transient organ contributes to overall fetal, infant and
adult health.
1.7 Cell death during human placental development
During normal placentation, a balance between proliferation, differentiation
and apoptosis is required to regulate cellular homeostasis and is essential for
maintaining proper placental function. While proliferation and differentiation of
trophoblast cells have been extensively studied, only recently has work begun to
address the importance of apoptosis during placental development [132, 173]. Cell
death in normal human placentation has been implicated in villous trophoblast
turnover and syncytialization, maternal immune tolerance and EVT invasion [174].
Cell death in villous trophoblast turnover and syncytialization
In the first trimester placenta, there is a low level of cell death, with the
primary site of apoptosis within the CTB cells [175]. In the second and third
trimesters, a shift in cell death susceptibility occurs, with higher levels of apoptosis
30
observed in ST cells [132]. It has been proposed that since these cells are
transcriptionally less active, they require constant replenishment with the cellular
machinery from overlying “stem” cytotrophoblast cells [144]. Based on several
markers of cell death, it was postulated that apoptosis is initiated in villus
cytotrophoblast cells at the time of fusion, then delayed during syncytialization.
Apoptosis is finalized just prior to the extrusion of apoptotic nuclei, which is observed
as placental shedding in the form of syncytial knots. Several Bcl-2 family members
and other apoptosis-associated molecules have been proposed to be involved in
regulating this process [104]. Among these, caspase-8 was recently shown to play a
crucial role in this process [89]. In addition, c-FLIP, a negative regulator of caspase-
8 activation, is expressed in human placentae [176] and has been postulated to
have a regulatory role in syncytial fusion [177]. It is further proposed that high
expression levels of Bcl-2 and Mcl-1 are maintained in both CTB [104] and ST [178,
179] cells in order to balance this unique pathway of cellular differentiation.
Cell death in maternal immune tolerance
Regulation of cell death in human EVT is not as comprehensively studied,
due to the difficulty of obtaining the appropriate tissue and cell types by placental
bed biopsies. Moreover, isolation of pure, primary EVT has been unsuccessful and
cell lines, although well characterized, only partially resemble the EVT phenotype
[177]. Perhaps the greatest advancements have surrounded the issue of maternal
immune tolerance, in an attempt to elucidate the mechanisms by which the maternal
immune cells do not reject the allo-antigenic fetal tissue. Extravillous trophoblast
31
cells are situated in a potentially precarious environment, as these cells invade the
decidua or the maternal spiral arteries and thus, are exposed to cytotoxic, maternal
immune cells. First-trimester EVT express high levels of FasL [180, 181], in what is
believed to be a protective mechanism against activated, Fas-expressing maternal
leukocytes. These data are supported by murine studies, where examination of
implantation sites in FasL-deficient mice revealed extensive infiltration and necrosis
of maternal neutrophils and macrophages [182]. Interestingly, early trophoblasts
have also been shown to express Fas [183]; however, these cells consistently
exhibit resistance to Fas-mediated death, in a mechanism that has only been
partially resolved, and may involve the caspase-8 inhibitor, c-FLIP [19].
Cell death during trophoblast invasion
During implantation, the blastocyst must appose and adhere to the uterine
wall, after which embryonic-derived cells begin invading the endometrium in a
mechanism which involves death of maternal cells [174]. Using both rodent and
human in vitro models, it has been demonstrated that endometrial cells are
susceptible to trophoblast-induced death during the invasion phase of implantation
[184, 185]. A possible mechanism involves the Fas/FasL system, as maternal
endometrial cells express Fas on their apical surface and human trophectoderm and
early trophoblasts have been shown to express FasL [185]. A similar mechanism
has been elucidated in mice; however, this system of implantation appears to utilize
the TNFR1/TNF-a pathway. This would allow the embryo to erode the uterine
32
epithelium, advance into the decidua and gain access to the maternal blood supply
[186].
Another important event during human and murine placentation is maternal
artery remodelling by the fetal-derived trophoblast cells. In a process that has been
studied both in vitro [187] and in vivo [188], maternal endothelial and smooth muscle
cells of the spiral arteries are replaced by endovascular trophoblast. This alters the
architecture of the vascular wall, increasing maternal blood flow to the placenta
[189]. In the absence of spiral artery transformation, nutrient and oxygen transport
to the fetus is compromised, leading to pathological conditions such as preeclampsia
and IUGR [189, 190]. During invasion of the human spiral arteries, maternal smooth
muscle and endothelial cells are replaced by EVT cells in a mechanism that has yet
to be resolved. Recent reports suggest that fetal-derived trophoblasts induce death
in these cell types via the Fas/FasL pathway [191, 192], in a process that is
mediated by maternal uterine natural killer cells [193].
1.8 Cell death during murine placental development
While it is now clear that apoptosis plays a functional role in placental tissue
morphogenesis, the underlying mechanisms coordinating cell death have not been
studied in this context. The localization and extent of cell death in the rodent
placenta and how this correlates to cell death patterns in human placenta remain
largely unknown. While some sporadic in vivo [194, 195] and in vitro [196]
observations have surfaced during investigations into other placental events, the
33
majority of what is known about cell death during murine placentation has largely
been derived through comparative gene knockout mouse studies.
Tumour suppressor genes and placental cell death
Tumour suppressor genes encode for proteins that are involved in cell cycle
regulation and cellular differentiation; such proteins are often referred to as
“gatekeepers”, inhibiting or permitting cell cycle progression, depending on the
internal and external status of the cell. A number of these genes — such as p53 —
have been implicated in promoting apoptosis in various cell types, as this outcome,
or cell senescence, is usually considered preferable to the propagation of a cell with
uncontrolled proliferative potential. The mouse placenta expresses a number of
these tumour suppressors, including p53, retinoblastoma (Rb), and phosphatase
and tensin homolog (PTEN).
The p53 tumour suppressor is a ubiquitously-expressed, multi-functional
transcription factor that is activated by DNA damage [197, 198] and other cellular
stressors, such as hypoxia [199, 200]. The primary function of this protein is to
induce G, arrest [201, 202] or apoptosis by activating the appropriate target genes.
In addition to its transcriptional activity, a novel p53-mediated apoptotic pathway was
recently described, suggesting that p53 translocates to the mitochondria, inducing
mitochondrial permeabilization via interaction with members of the Bcl-2 and BH3-
only family [203, 204]. The transcriptional and apoptotic potential of p53 in murine
placental celis have been demonstrated both in vivo and in vitro. p53 has exhibited
involvement in triggering the apoptotic pathway in early, proliferating trophoblast
34
cells with compromised genomic stability [205, 206]. In vivo studies of the effects of
DNA-damage-inducing agents on rat placentation revealed that cells within the
labyrinth appear most susceptible to p53-mediated apoptosis, as evidenced by
increased levels of active caspase-3 [207, 208]. Lastly, a recent report by Soloveva
and Linzer [155], demonstrates that the loss of p53 in differentiating murine
trophoblast stem (TS) cells renders them not only resistant to DNA-damage-induced
apoptosis, but also allows them to bypass the critical G; checkpoint. This is
supported by the report that extraembryonic cells, but not embryonic cells, were
resistant to p53-dependent cell death after DNA damage [209]. p53-deficient mice
are viable, but cells derived from these animals demonstrate higher proliferation
rates in culture [210]; however, the growth dynamics of trophoblast-derived cells is
currently unknown.
Retinoblastoma (Rb) protein is also a tumour suppressor, with a prominent
role in cell cycle regulation. The phosphorylation state of Rb correlates with its
functional capacity: phosphorylation is maximal at the start of S phase (i.e. in
proliferating cells) and lowest after mitosis and entry in G, (i.e. in quiescent cells);
hence, the hypophosphorylated form of Rb suppresses cell proliferation. It was
recently demonstrated that hypophosphorylated Rb predominates in murine TS cells
deprived of Fgf-4 (a required growth factor for TS cells) and hyperphosphorylated Rb
is found in actively growing TS cells [155]; however, all forms of Rb protein were
observed to decrease in differentiating TGC in vitro [155]. Initial studies producing
Rb-null mice revealed that these mice die between embryonic days 13.5-15.5,
displaying abnormalities in erythropoiesis and central nervous system, due to
35
excessive apoptosis, failed differentiation and disruption of the cell cycle [211-213].
Additionally, it was later reported that Rb mutant placentae exhibit increased
numbers of trophoblast cells in the labyrinth, leading to disrupted architecture of this
placental region and resulting in decreased placental vascularization and transport
[146]. These data indicate that Rb mutant placentae appear to have an
unprogrammed proliferation defect within the labyrinth, offsetting the balance
between the cell death and proliferation pathways. In order to determine whether
the embryonic phenotype was secondary to a placental defect, tetraploid
aggregation and conditional knockout approaches were employed to provide Rb-
deficient embryos with wildtype placentae. Under these conditions, the knockout
embryos were carried to term, but died shortly after birth [146], suggesting that the
majority of embryonic phenotypes in Rb-deficient embryos are caused by a
dysfunctional placenta and are therefore, not due to a cell-autonomous Rb
requirement by the embryo. Rb family members bridge the cell death and cycle
pathways through the direct repression of E2F/Dp transcription factors [214]. Free
E2F/Dp heterodimers stimulate entry into the S phase of the cell cycle and either
subsequent proliferation or apoptosis, depending on the cellular context [215].
Recently, it was reported that Dp1-deficient embryos die by embryonic day 12.5 and
demonstrate increased rates of apoptosis in early extraembryonic cells [216].
Moreover, embryonic lethality caused by Dp1 deficiency was shown to be largely
due to placental defects, as late-gestation Dp1-null fetuses were obtained after
placental rescue [216].
36
PTEN is a tumour suppressor that has been shown to inhibit cell migration,
cell spreading and focal adhesion formation through interactions with focal adhesion
kinase [217, 218]. Additionally, PTEN has been shown to negatively regulate
phosphoinositide-dependent kinase 1 (PDK1), which phosphorylates and activates
protein kinase B (PKB/Akt1), triggering a well-established survival pathway [219,
220]. PTEN is ubiquitously expressed in embryonic day 7.5 mouse embryos and its
inactivation in the mouse causes embryonic lethality at d9.5 [221, 222]. Knockout
embryos demonstrate regions of increased proliferation, including the allantois, the
expansion of which is hypothesized to inhibit chorioallantoic fusion and therefore,
cause embryonic death [221]. Interestingly, murine trophoblast and endothelial cells
have been demonstrated to express PKBo/Akt1, and the consequences of
PKB/Akt1-deficiency include reductions in the decidual basalis, glycogen-containing
SpT and vascularization [223]. These defects indicate a deficiency in placentation,
leading to the observed fetal growth reduction, neonatal lethality and diminished life
span after exposure to genotoxic stress [223]. Lastly, it has also been shown that
PKB/Akt1 signalling is involved in differentiation of murine TS cells to TGC in vitro
[224]. Since TGCs in the mouse placenta are involved in the production of
numerous protein and steroid hormones, it is possible that reduced placental and
fetal growth may be due to the impaired differentiation of this cell type.
Cell death-associated genes and placentation
While many cell death regulatory molecules are expressed in the mouse
placenta, their roles in this organ have not been functionally characterized. Bruce
37
(baculovirus inhibitor of apoptosis repeat-containing [BIR] ubiquitin-conjugating
enzyme) is a large (528 kDa) protein that has both an N-terminal BIR domain and a
C-terminal ubiquitin-conjugating domain (UBC); these regions provide Bruce with
both antiapoptotic [225-227] and ubiquitylation capabilities [227, 228]. There are
several inhibitor of apoptosis (IAP) proteins, including Bruce, which function as cell
death antagonists by suppressing pro-apoptotic proteins such as Smac and active
caspase-9 [227, 228]. The murine Bruce gene is highly conserved, as human
APOLLON shares 92% identity with Bruce and has been demonstrated to confer
chemotherapeutic resistance to certain cancer cells [226]. Lotz et al. [229] reported
that Bruce is highly expressed in the labyrinth and SpT of the placenta; lower
expression levels were observed in TGCs. Analysis of earlier developmental stages
revealed that Bruce can also be detected in the chorion, within the cells of the EPC
and in early TGCs as well as in the late gastrula stage embryo [230, 231].
Three separate groups of investigators have produced Bruce-deficient mice,
with two groups observing a trophoblast proliferation-related phenotype and no
alterations in cell death [229, 230]. The third group also observed proliferation
defects but additionally reported increased rates of apoptosis in Bruce-deficient
placentae [231]. Loss of Bruce leads to embryonic and/or perinatal growth reduction
and lethality, which can likely be attributed to the observed placental defects.
Proliferation was severely reduced in the SpT [229, 230], and was diminished in the
labyrinth [229]. In contrast, Ren et al. [231] reported defects in trophoblast cell
death, with elevated levels of Bax, Bak and caspase-2, and activation of the
mitochondrial cell death cascade in embryonic fibroblasts obtained from mutant
38
embryos. Moreover, p53 expression was also shown to be elevated in Bruce-
deficient placentae, particularly in SpT cells, and silencing of p53 and Bruce
expression in cell lines resulted in improved cell viability [231]. Thus, p53 appears to
acts as a downstream effector of Bruce, and in the absence of Bruce,
mitochondrially-mediated apoptosis ensues [231]. The conflicting results of these
studies is perhaps, not so unexpected in hindsight. Bruce is a chimaeric molecule,
with both ubiquitylation and apoptois-inhibiting capabilities, underscoring the
multifunctional nature of this protein. Yeast homologs of Bruce have likewise been
shown to be involved in cell division [232, 233]. On the other hand, as previously
stated, Bruce is also clearly associated with regulation of the apoptotic pathway and
further molecular analysis into the nature of this enigmatic — yet exciting — molecule
in the right cellular context is required in order to further elucidate the function of
Bruce during mammalian placentation.
Daxx (Fas death domain-associated protein) was initially reported as a highly
conserved protein, interacting with the intracellular domain of Fas and enhancing
Fas-mediated apoptosis in overexpression studies [234]. As is the case with Bruce,
Daxx is a multifunctional protein with seemingly contradictory functions. It has been
shown to be involved in both extrinsic (TGF-B -mediated) and intrinsic (p53-
dependent DNA damage) apoptosis pathways [235, 236]. In addition to these cell
death functions, Daxx is also capable of transcriptionally repressing CRE, E2F1,
Sp1, NF-«B and the androgen receptor [237, 238], demonstrating further potential in
modulating cellular behavior. Daxx is expressed in a number of murine [239] and
human tissues [240], including the placenta. Daxx deficiency in mice leads to
39
embryonic lethality by day 9.5 and both embryonic and extraembryonic lineages are
diminished in comparison to wildtype littermates, marked by increased rates of
apoptosis by day 7.5 and day 8.5 [241]. This enhanced apoptosis was unexpected,
since Daxx had until then, only been associated with promoting apoptotic events in
the cell; however, further investigation revealed that Daxx mutant embryonic stem
(ES) cell lines also had elevated rates of apoptosis. It was later revealed that a
similar Daxx deletion triggered cell death by stimulating the JNK/p38-Bim-Bax
pathway, leading to the activation of caspase-9 and caspase-3 [242]. Lastly, Daxx
has recently been reported to play a role in viral protection, as Daxx-null fibroblast
cell lines demonstrated enhanced viral gene expression compared to Daxx-
complemented cells [243]. Therefore, it is intriguing to speculate that in addition to
the role of Daxx as a regulator of cell death in the placenta, it may also be involved
in protecting the trophoblast and hence, the fetus, from viral invasion.
Prostaglandin Fz (PGF2a) receptor (FP) is a G-protein-coupled receptor that
has been shown to induce the apoptotic cascade by activating caspase-8 in luteal
cells [244]. Interestingly, FP lacks an intracytoplasmic region possessing any of the
traditional death or caspase-recruiting domains that characterize other, typical death
associated receptors. Prostaglandin Fz, receptor is highly expressed in the uterus
[245], but it has also been shown to be expressed in the mouse [246] and human
[239] placenta. Homozygous deletion of FP resulted in developmentally normal and
viable mice, but FP-deficient females failed to deliver their fetuses at term, leading to
in utero death, followed by resorption [247]. No changes were detected in mutant
placental and decidual weights, nor were there any disparities in placental cell death
40
patterns; however, elevated decidual cell death over gestation was noted [194].
Further characterization of phenotype revealed alterations of decidual cell death
patterns once post-term fetuses were categorized as either live or dead. Elevated
decidual cell death in dead fetuses was associated with alterations in the Bax:Bcl-2
ratio and increased active caspase-3 levels [248]. Given these observations, it was
hypothesized that decidual cell death was necessary for normal term delivery of the
conceptus and that a Bax:Bcl-2 “rheostat” is involved in regulating apoptosis in the
postterm placenta [248]. On the contrary, upregulation of Bcl-2 was reported in the
decidua of abortion-prone mice, perhaps serving as a compensatory or protective
mechanism [249], especially considering the premature “delivery” of these preterm
placentae.
It is evident that cell death plays a key role in the appropriate maturation of
the placenta and that pro- and anti-apoptotic expression patterns can be
manipulated in the fetal-placental-maternal unit in order to optimize the uterine
environment for healthy gestation.
1.9 Maternal exposure to cigarette smoke, polycyclic aromatic hydrocarbons and placentation
Polycyclic aromatic hydrocarbons (PAH) such as 7,12-
dimethylbenz(a)anthracene (DMBA) and benzo(a)pyrene (BaP) are released into the
environment as a result of incomplete combustion of fossil fuels; however, the
primary route of human exposure to these compounds is cigarette smoke [250].
Epidemiological studies have revealed that exposure to pollution and smoking during
41
pregnancy is associated with many adverse outcomes, including intrauterine fetal
growth restriction, preterm delivery and increased perinatal mortality [251-253].
However, the association between exposure to tobacco products and miscarriage
has yet to be firmly established. While some studies have reported an increased
risk of spontaneous abortion due to smoking during natural or assisted conception
[254-256], others have reported that no significant association exists [257]. These
inconsistencies may be due to inaccurate self-reporting on the part of the subjects,
the varying numbers of cigarettes smoked from subject to subject and the time at
which the miscarriage occurred, as earlier abortions may go undetected.
Another smoking-related pathology that has been observed in human
populations is delayed conception and infertility. Several epidemiological studies
have reported reduced pregnancy rates in women who were currently smoking,
compared to women who were never smokers and ex-smokers (i.e. those who had
ceased smoking for one year before attempting conception) [258-260]. One study
further demonstrated that women exposed to environmental tobacco smoke were
more likely to fail to conceive within six months, compared to non-exposed women
[261].
Cigarette smoking during pregnancy also influences the placental
vasculature, resulting in reduced dimensions of the fetal capillaries [262, 263] and
increased uterine artery resistance [264]. This is consistent with a reduction of
surface area and length of villous capillaries in placenta of smokers at term [265], as
well as the observed decrease in ST apoptosis [175, 266], likely a consequence of
abnormal trophoblast turnover. The observed reduction in fetal capillary dimensions,
42
possibly due to insufficient remodelling of maternal spiral arteries into vessels of low
resistance, affects placental blood flow [267]. Reduced placental perfusion has
been implicated in poor exchange of gases and nutrients between fetus and mother
[268], possibly leading to IUGR.
Several reports have indicated cellular and trophoblast differentiation defects
in placentae of heavy smokers accompanied by alterations in the cell death rates
[175, 269]. Cytotrophoblast cells, isolated from first trimester placenta of smoking
mothers, have reduced invasive potential and poor differentiation capabilities in vitro
[269]. This is accompanied by an increase in the number of columns of
cytotrophoblast origin that failed to reach the uterus [270]. Gruslin et al. [175],
reported an increased rate of apoptosis in smokers during first trimester, but
decreased rates at term. These findings suggest that trophoblast cells from first and
third trimester placenta may differ in cell death susceptibility, which may be due to
changes in the expression of different sets of cell death genes.
Cigarette smoke contains many different chemical compounds, most of which
have unknown biological activity. While some studies determined nicotine as the
cause of uteroplacental insufficiency [269, 270], these predictions were recently
questioned since no adverse maternal or fetal outcomes were observed in patients
undergoing nicotine replacement therapy during pregnancy [271]. Thus, it was
concluded that the myriad of cellular and molecular abnormalities observed in
placentae and newborns of smoking mothers could be caused by exposure to one or
more of the other thousands of chemicals found in cigarette smoke or by their
metabolic by-products. This is consistent with observations of significant
43
accumulation of PAHs in placenta [272], leading to DNA adduct formation and
altered activity of harmful downstream enzymes induced by PAHs in placental
samples of either smokers [273], or women living in areas of significant
environmental pollution [252, 274].
Animal studies using various types and sources of PAHs have also shown
that exposure to these toxins can lead to unfavourable reproductive outcomes. It
was recently shown in rats, that mid-gestation inhalation of aerosolized BaP resulted
in decreased fetal survival in a dose-dependent manner [275]; similar results have
also been reported in pregnant rats [276] and mice [277] exposed to BaP.
Resorption of the entire litter was observed in pregnant mice orally exposed to
carbon black oil, which is a petroleum refinery by-product, containing several classes
of hydrocarbons, including PAHs [278].
While there is a plethora of animal studies involving the exposure of pregnant
animals to PAHs, there is virtually no data on the reproductive outcome after
chronic, maternal exposure to PAHs. Previous studies in rats have determined that
after intravenous BaP exposure, this chemical demonstrated a long half-life in a
number of different tissues [279], and that chronic, oral exposure of BaP (50-100
mg/kg) leads to persistence of DNA adducts in liver and lung tissue [280].
Therefore, it would appear that PAH exposure prior to pregnancy has long-lasting
effects, likely due to accumulation of these compounds and their metabolites in
various tissues.
44
1.10 The aryl hydrocarbon receptor
There are several possible ways that PAHs can alter cell function at the
molecular level. These compounds are capable of directly altering DNA structure via
formation of DNA adducts [281] resulting in DNA mutations in affected cells. In
addition, PAHs interact with aryl hydrocarbon receptor (AhR), a member of the basic
helix-loop-helix family of transcription factors, having a broad range of tissue
expression [282]. AhR is an intracellular receptor that binds aryl hydrocarbons and
plays a major role as a xenobiotic sensor, inducing expression of metabolic enzymes
to rid the cell of these potentially harmful compounds. In the absence of ligand, AnR
exists in the cytosol associated with heat shock protein 90 (HSP90) and XAP2, an
immunophilin-related protein (Figure 1.4). Extracellular ligands, such as PAHs,
diffuse through the plasma membrane and bind to AhR, causing a conformational
change that exposes a nuclear localization sequence. The entire complex
subsequently translocates to the nucleus, whereupon the AhR-ligand complex
dissociates from the associated proteins and binds to aryl hydrocarbon nuclear
translocator (Arnt). At this point, the AnR-Arnt complex is transcriptionally active and
binds to specific DNA sequence called dioxin response, or AnR response elements
(DREs/AHREs), resulting in the expression of Phase | and Phase I! detoxifying
enzymes [283]. AhR appears incapable of homodimerizing and partners only with
Arnt. This is supported by in situ hybridization studies of murine embryos over
gestational timepoints, where Arnt was revealed to have overlapping expression in
those tissues expressing AhR [284].
45
a .
LO ligand “ binding
Lo OS NS
.
\ |
\ eo ° j
‘Transcription of PhaseJ’and Phase Ii \ f detoxification enzymes; \ other transcribed genes include those - 3 \ ‘ involved in cell cycle, differentiation and growth. control, apoptosis
~N 4
Nucleus
Figure 1.4 Schematic representation of the aryl hydrocarbon receptor pathway.
46
A great deal of cross-talk exists between AhR and other cellular pathways
signalling proliferation [285], cell cycle arrest [286], hypoxia [287] and response to
hormones [288], leading to a diverse range of biological outcomes. While the
majority of studies investigating ANR function have revolved around its ligands, it has
become increasingly clear that AnR does not need an exogenous ligand to activate
its signaling pathway. This was initially observed during studies in murine embryonic
palate development [289] and later supported by targetted gene knockout of AHR.
Homozygous mutant mice are viable and fertile, but are smaller, exhibit reduced
fecundity and have hepatic, hematopoietic and immune defects [290, 291]. In
addition, AhR-deficient mice are resistant to BaP and dioxin exposure. Currently,
there is no information as to a possible placental phenotype due to AMR deficiency;
however, both Arnt and AhR mRNA transcripts exist in a number of different female
reproductive tissues in both humans and rodents [292-295], with high expression
levels being reported in the placenta [292, 293, 296].
In contrast to AhR, Arnt has multiple binding partners and is involved in
various signalling pathways, regulating cellular responses to hypoxia, angiogenesis
[297] [298] and embryonic development [299]. Targetted gene knockout of Arnt in
mice resulted in embryonic lethality at d10.5, exhibiting defects in vascularization
and embryonic development [298, 300]. Moreover, Arnt-deficient placentae were
reported to have greatly reduced labyrinth and SpT, and increased numbers of
TGCs [300], suggesting that Arnt may play a role in trophoblast cell fate. In light of
the results reported after gene knockout studies, an additional role for AnR during
development of both embryonic and adult tissues was proposed. Robles et al. [301]
47
demonstrated that AnR was required for normal ovarian germ cell endowment, as
AhR-deficient mice had twice the follicular reserve as their wildtype counterparts. In
addition, cardiac hypertrophy [302] and patent hepatic ductus venosus [303] were
reported in adult mice deficient in ANR. Moreover, mice transgenic for a
constitutively active AnR have a reduced lifespan and are prone to gastric tumours
[304]. However, while the existence of an AnR-regulated pathway during normal
development appears likely, the identities of possible endogenous ligands and
developmental cues remain enigmatic.
The aryl hydrocarbon receptor has been postulated to be highly tolerant to
evolutionary adaptations. A number of studies have reported the existence of one
copy of AhR in invertebrates such as C. elegans [305], D. melanogaster [306] and
several mollusks (reviewed in [307]); however, the AhR found in invertebrates does
not bind the typical ligands seen in vertebrates. Interestingly, non-mammalian
vertebrates (e.g. birds, reptiles, fish, amphibians) possess two copies of AhRs that
mediate xenobiotic sensing and activate transcriptional machinery resulting in the
profound phenotypic consensequences due to dioxin exposure that are observed in
these animals (reviewed in [308]). The mammalian genome has one copy of AhR,
which has also exhibited diversity at both the gene and protein level. Human AhR,
in addition to some of its target genes such as CYP 1A1 and GST M1 [809], has
been shown to be highly polymorphic (reviewed in [283, 310]). The consequence of
such genetic polymorphisms in AhR results in inter-individual variations in PAH
metabolism [309] and unpredictable susceptibilities to diseases such as cigarette-
smoking-related lung cancer [311] and hypertension [312]. Both mouse and rat AhR
48
exhibit polymorphic gene sequences (reviewed in [283, 310]), yielding the highly
variable phenotypes that are observed after dioxin or PAH exposure in these
animals. In fact, four murine AhR alleles exist, originally discovered in “dioxin-
resistant” DBA/2 and “dioxin-sensitive” C57BI/6 mice [313]. Examination of the AhR
gene in 13 mouse lines confirmed the identification of these four alleles and
evolutionary analyses yielded a high tolerance to nucleotide substitution in murine
AhR [814]. Thus, AhR is subject to a high degree of evolutionary pressure within a
number of evolutionarily divergent organisms.
1.
49
HYPOTHESES
Murine placental cell death is a regulated event, required for optimal
placentation and dysregulation of this process affects embryonic and fetal
development.
Chronic maternal exposure to polycyclic aromatic hydrocarbons prior to
conception will interfere with normal cell death, perturbing normal placental
development, which will have deleterious consequences on the offspring.
The aryl hydrocarbon receptor and its downstream, pro-apoptotic target, Bax,
are involved in regulating murine placental cell death and deficiencies in
these genes will rescue the observed PAH-induced embryonic and fetal
phenotypes.
50
CHAPTER 2
MURINE PLACENTAL CELL DEATH EXHIBITS AN ORGANIZED PATTERN
OVER GESTATION AND PLACENTAL DEFICIENCY OF PRO-APOPTOTIC BAX
LEADS TO ALTERED LABYRINTHINE ARCHITECTURE AND IUGR
51
CHAPTER 2: Murine placental cell death exhibits an organized pattern over gestation and placental deficiency of pro-apoptotic Bax leads to altered labyrinthine architecture and IUGR
2.1 Abstract
While cell death in the human placenta has been recognized as a physiological
event, virtually no studies have been done on the mouse placenta. Herein, we
report the results of a systematic and quantitative examination into cell death
patterns in both ICR and C57BV/6 placentae, over gestation. Furthermore, we
investigated the effects of Bax deficiency on murine placentation and the
consequent outcome of this deletion on the fetus. Over gestation, ICR and C57BI/6
placentae exhibited TUNEL-positive patterns similar to those observed in human
placentae, with sporadic, infrequent death observed in early placentae, which
increased towards term. The most striking observation was the organized pattern of
TUNEL-positive cells surrounding the vessels of the labyrinth at mid-gestation, with
an apparent role in remodeling the vasculature of this region. While cell death
patterns were similar for both strains of placentae examined, C57BI/6 placentae
demonstrated greater numbers of dead cells in almost all placental regions, starting
at d13.5. Bax, a pro-apoptotic, Bcl-2 family member, immunolocalized to a subset of
trophoblast giant cells (TGCs) and to cells within the labyrinth. Bax deficiency in the
mouse placenta resulted in an altered labyrinthine architecture, leading to fetal
intrauterine growth restriction and additionally, revealed a role for Bax in the
programmed cell death (PCD) of trophoblast giant cells (TGCs).
52
2.2 Introduction
Programmed cell death has been shown to be an important part of a large
number of biological processes, including embryogenesis, organogenesis, tissue
remodeling and normal cellular homeostasis [315]. Hallmark features of apoptosis
include cell/nuclear shrinkage, chromatin condensation, DNA fragmentation and
membrane blebbing, leading to the production of apoptotic bodies, which are
efficiently eliminated by phagocytosis [316]. However, cells do not always die along
the apoptotic pathway and may exhibit signs of autophagy (characterized by
autophagic vacuolization of cytoplasmic contents and lack of chromatin
condensation), necrosis (cytoplasmic swelling, plasma membrane rupture, moderate
chromatin condensation, leaky nuclear envelope), or may display combined features
of several types of cell death, such as aponecrosis or apoptosis accompanied with
autophagy (for reviews, see [73, 317]. Alterations in cell death rates are known to
have pathological consequences, with a deficiency in cell death resulting in cancer
or autoimmune disorders and an augmentation or acceleration of cell death leading
to degenerative diseases. Thus, a fine balance in the loss and production of new
cells is essential for all organs, particularly for those that depend on tissue
remodeling.
During normal placentation, proliferation, differentiation and apoptosis
contribute in a balanced fashion to maintain homeostasis and proper placental
function. While proliferation and differentiation of trophoblast cells have been
extensively investigated, only recently have studies begun to address the
importance of cell death during normal and abnormal placentation in human [131,
53
132]. In a healthy placenta, cell death has been implicated in regulation of
trophoblast turnover. Syncytiotrophoblast cells require constant replenishment by
overlying “stem” cytotrophoblast cells [144] and this renewal is driven by molecules
regulating the cell death cascade. It has been postulated that apoptosis is initiated
in villus cytotrophoblast cells at the time of fusion, delayed during syncytialization,
then subsequently finalized just prior to the extrusion of apoptotic nuclei [104], which
are termed syncytial knots. This process of cell fusion uniquely provides the
transcriptionally quiescent ST with new materials to maintain the maternal-fetal
exchange unit. Only recently has a functional link between cell death and placental
vasculogenesis been established in humans [318]; however, the localization and
extent of cell death in the rodent placenta, and how this compares with cell death
patterns in the human placenta remain largely unknown.
During invasion of the spiral arteries, maternal smooth muscle and endothelial
cells are replaced by EVT cells in a mechanism that has still yet to be resolved.
Recent reports suggest that fetal-derived trophoblasts induce death in these cell
types via the Fas/FasL pathway [191, 192], in a process that is mediated by
maternal uterine natural killer cells [193]. Extravillous trophoblast cells are situated
in a potentially precarious environment, as these cells invade the decidua or the
maternal spiral arteries and thus, are exposed to cytotoxic, maternal immune cells.
In what is believed to be a cytoprotective mechanism against Fas-expressing
maternal leukocytes, first-trimester EVT express high levels of FasL [180, 181].
Interestingly, early trophoblasts have also been shown to express Fas [183];
however, these cells consistently exhibit resistance to Fas-mediated death. On the
54
contrary, a recent study reports the susceptbility of EVT to interferon-y-induced
death — a cytokine produced by maternal uNK cells — impeding EVT invasion and
maternal spiral artery remodelling [319]. This is supported by studies of tubal
pregnancy, where decreased rates of EVT apoptosis have been attributed to the
altered immune microenvironment [320].
Comparative studies between mouse and human placentae have
demonstrated striking similarities in the molecular and cellular framework during
development of this tissue. Between 7.5-9.5 days post coitum, the developing EPC
undergoes major morphological remodeling, resulting in the formation of three
distinct cellular regions, each with unique morphology and function (for review [136]).
The fusion of the allantois with the chorion and subsequent branching, establishes a
network of villi surrounded by small canals collectively referred to as the labyrinth.
This region is responsible for gas and nutrient exchange, and thus bears a similarity
to floating chorionic villi in human. The junctional zone consists of variable-sized
SpT cells with the capability of differentiating into secondary TGCs and GlyTs. Due
to the expression of several gene markers, as well as to their spatial distribution, the
cells of this region are considered to be analogous to human cytotrophoblast cells
found in columns [158]. The two invasive trophoblast cell types in the mouse
placenta are GlyTs, a cell having distinct morphology but unknown function, and
TGCs. These latter cells invade the endometrium and are positioned in direct
contact with the maternal decidua; thus, TGCs are analogous to human extravillous
trophoblast cells. Trophoblast giant cells have distinctively large, polyploid nuclei
and are efficient in producing several key regulatory, luteotropic and lactogenic
55
hormones, as well as angiogenic factors [159]. In addition, it was recently reported
that a subset of specialized murine TGCs are capable of invasion and remodeling
maternal spiral arteries [147], a physiologically important event that also occurs
during human placentation.
Here, we report the results of a systematic analysis of the temporal and
spatial distribution of dying cells throughout gestation in the placentae of two
different strains of mice. In addition, we have established the expression profile of
several cell death-related markers in the placentae of both mouse strains and we
describe a placental phenotype in mice deficient in Bax, a pivotal, pro-apoptotic Bcl-
2-related gene.
2.3 Materials and Methods
2.3.1 Animal housing, mating and tissue collection
Six-week-old ICR, (Harlan, Indianapolis, IN, USA), C57BI/6 (National Cancer
Institute, Frederick, Maryland, USA) and Bax heterozygous (C57BI/6 [49]) virgin
females were mated with the appropriate male stud (i.e. ICR, C57BI/6 and Bax
heterozygous males) of proven fertility. Gestational age was determined based on
the presence of a vaginal plug, with the morning of detection being day 0.5 (d0.5)
post coitum (pc). Animals were maintained in a controlled room with a 12h light: 12
h dark cycle and allowed ad libitum access to rodent chow and water.
Pregnant ICR and C57BI/6 females (from d7.5-d18.5) were euthanized by
cervical dislocation and the uterine horns were removed. Approximately 3-5
56
conceptuses were collected with the uterine tissue still intact and immersion-fixed in
ice-cold 10% phosphate-buffered formalin for 24 hours. Fixed tissue were
subsequently washed 2 x 1 hour in PBS and stored in 70% ethanol at 4°C. The
remaining uterine horn was placed in phosphate-buffered saline (PBS) and the
uterine tissue was torn open with forceps and conceptuses teased out. Decidual
tissue was removed from d7.5 and d8.5 EPC and discarded, while the decidua was
left intact on d9.5-d18.5 placentae; after determining normal development by
morphological assessment, embryos/fetuses were discarded. Ectoplacental cones
from the same dam were pooled in order to have enough tissue for immunoblotting
analyses. Tissues for immunoblotting and caspase-3 assays were stored at -80°C.
Bax heterozygous females were euthanized at d15.5 and d18.5; uterine horns
were collected in PBS, and conceptuses were freed from uterine tissue as described
above. Wet weights of fetuses and placentae (with attached decidua) were recorded
and placentae were either frozen on dry ice or fixed in ice-cold, 10% phosphate-
buffered formalin for 24 hours. A piece of fetal forelimb tissue was removed,
washed in PBS, placed on dry ice and stored at -20°C for genotyping, as previously
described [321]. All animal experiments were conducted using protocols approved
by the Animal Care Committee at the Samuel Lunenfeld Research Institute, Mount
Sinai Hospital.
2.3.2. Terminal deoxynucleotidyl transferase dUTP nick-end labeling
Three healthy conceptuses (d7.5) or placentae (d9.5-d11.5, d13.5, d15.5 and
d18.5) from three different ICR or C57BI/6 dams were embedded in paraffin using
57
routine histological techniques; d7.5 conceptuses were embedded whole, while
later-gestation placentae were cut slightly lateral to the midline and the larger half
was embedded to obtain transverse sections. Tissue blocks containing d7.5
conceptuses were serially sectioned at 5 um thick and examined under the
microscope before staining. Those sections containing the EPC at the approximate
midline and sections corresponding to 50 and 100 um distant to one side of the
midline, were chosen for each sample to be used for TUNEL staining. Tissue blocks
containing placentae were trimmed until just before the midline (estimated by the
presence of the umbilical cord) and 5 um serial sections were cut until approximately
150-200 ym of tissue had been sectioned. Those sections at midline, and at 50 ym
and 100 um from midline were used for TUNEL staining.
Sections were deparaffinized and treated with 10 g/mL proteinase K
(Invitrogen, Burlington, ON, Canada) in PBS for 13 minutes, followed by brief
washes with MilliQ water and PBS. Endogenous peroxidase was quenched in 3%
H2O2 in methanol for 30 minutes, slides were washed in PBS and pre-equilibriated
for 10 minutes at room temperature in a solution of 1x One-Phor-All PLUS buffer
(GE Healthcare, Baie d'Urfe, QC, Canada) supplemented with 0.1% Triton X-100
(Sigma, Oakville, Ontario, Canada). TUNEL reaction mixture was prepared with the
following final concentrations, diluted in 0.1% Triton X-100: 1 x One-Phor-All PLUS
buffer, 10 uM biotin-16-dUTP (Enzo Life Sciences, Farmingdale, NY, USA), 1 uM
dATP (Fermentas, Burlington, ON, Canada) and 20 IU of terminal deoxynucleotidyl
transferase, FPLC™ pure enzyme (GE Healthcare). Sections were incubated with
the TUNEL reaction mixture in a humidified chamber for 90 minutes at 37°C and
58
then washed with PBS. Streptavidin-horseradish peroxidase reagent (Vector
Laboratories, Burlingame, CA, USA) was used for detection of incorporated,
biotinylated nucleotides and the colour reaction was developed using
diaminobenzidine (DAB) substrate (Sigma). Sections were counter-stained with
methyl green, dehydrated and mounted. Histomorphometric analyses were done on
each placental section, with the researcher blind to the strain of mouse and
gestational timepoint, using a Zeiss 9901 microscope, a Retiga 1300 camera and
BioQuant® Software. For d7.5, the conceptus was divided into regions of
mesometrial decidua, anti-mesometrial decidua and EPC; all TGCs and allantoic
cells were counted in each section. For all other timepoints, placental regions were
divided into chorionic plate (CP) and labyrinthine regions, the junctional zone (area
between the labyrinth and giant cell border) and the maternal compartment (area
between the giant cell border and the myometrium; see Figure 2.1). All TGC ells
were counted for each section, except for those that were contained within the
extreme lateral edges of the placenta, adjacent to the decidua parietalis. Tissue
areas were determined at 25x, 100x or 500x magnification, depending on the size of
the region; TUNEL-positive cells were counted at 500x magnification, scanning each
section in its entirety. If a group of dead cells in the maternal compartment
contained greater than nine TUNEL-positive cells, these were considered to be focal
points of death and the area of these foci was determined at 500x magnification.
The rate of this type of death was expressed as a percent of the area exhibiting
TUNEL staining, over the total area of the tissue in the maternal compartment. The
different data sets for the three sections were averaged to obtain final areas and cell
59
Maternal compartment
TGC border
Junctional zone
Labyrinth
Chorionic plate
i oe : 1mm f sANS.
d15.5 ICR placenta outlining approximate regions of measurement for d10.5 - d18.5 placenta
Figure 2.1 Low-magnification placental section of d15.5 ICR placenta,
demonstrating various regions of placenta used for histomorphometry.
Masson trichrome-stained section was used for this diagram as methyl green-
stained sections were too faint at low magnification for visualization.
60
death numbers for each placenta. Photomicrographs were taken using a Leitz
DMRXE microscope, a Sony DXC-970MD camera and Northern Eclipse® software.
2.3.3 Giant cell counts in Bax-deficient placentae
Formalin-fixed Bax WT and KO littermate d15.5 and d18.5 placentae were
embedded in paraffin using routine histological procedures; an approximately
midline section was labeled using the TUNEL procedure described above. Each
section was examined blind using a Zeiss 872 E compound microscope, at 400x
magnification and the number of TUNEL-positive and -negative cells per placental
section was counted.
2.3.4 Immunohistochemistry and lectin histochemistry
Sections were deparaffinized in xylene, rehydrated and underwent microwave
antigen retrieval in 10 mM citrate buffer, pH 6.0. Sections were allowed to cool
down to room temperature, washed, then blocked with 10% horse serum + 10%
BSA in PBS with 0.1% Tween 20 (PBST). Anti-active-caspase-3 antibody (Cell
Signalling, Danvers, MA, USA) was diluted 1:500 in 5% horse serum + 5% BSA in
PBS. Slides were then held at 4°C overnight, washed in PBS, followed by a 2-hour
incubation at room temperature with biotinylated anti-rabbit antibody (1:200 dilution
in 5% horse serum + 5% BSA) from a VectaStain ABC kit (Vector Labs). The ABC
solution was prepared according to the manufacturer’s instructions and detection
61
using DAB substrate was done as described above, followed by counterstaining with
hematoxylin.
Immunofluorescence using anti-Bax NT antibody (Upstate, Lake Placid, NY,
USA) was similar to the method described above, except an autofluorescence
quenching step was added before blocking (slides held in 0.1% Sudan Black in 70%
ethanol for 30 minutes, followed by washes in PBS) and the step to quench
endogenous peroxidase was omitted. In addition, streptavidin, conjugated to
fluorescein isothiocyanate (FITC; Chemicon, Temecula, CA, USA) was used for
detection, nuclei were counterstained with 4,6-diamidino-2-phenylindole (DAPI;
Sigma) and slides were mounted with anti-fade medium (Vector Labs). Sections
were examined and imaged on a deconvolution microscope (Olympus IX70, Applied
Precision Inc., lssaquah, WA, USA), using FITC and DAPI filters. Images were
acquired using DeltaVision Software (Applied Precision Inc., Issaquah, WA, USA)
and the DAPI channel was assigned a red wavelength to allow for greater resolution
of photomicrographs.
Lectin histochemistry was used to identify the fetal endothelium. The
methodology used was similar to that described for immunohistochemistry, except
antigen retrieval was omitted and secondary antibody was not needed. Instead,
sections were blocked and probed with 50 ug/mL biotinylated Bandeiraea
simplicifolia (Sigma) for 1 hour at room temperature. This was followed by
peroxidase quenching using 1% H2O2 in PBS, then washes in PBS. Detection of
reaction using the ABC complex and DAB substrate was done as described above.
62
Images of sections after immunohistochemistry and lectin histochemistry were taken
using the same instrumentation as that described for TUNEL photomicrography.
2.3.5 Caspase-3 enzyme assay
Enzymatic activity of caspase-3 in murine placental tissues was assessed
using the Caspase-3 Cellular Activity Assay Kit PLUS (Biomol, Plymouth Meeting,
PA, USA). Briefly, d15.5 placentae from both ICR and C57BI/6 mice (1 placenta
from each of n=4 dams) were dissected into either maternal-enriched or fetal-
enriched fractions (Figure 2.10a), weighed and homogenized in cell lysis buffer at a
ratio of 1 mg tissue: 5 wL lysis buffer. Protein concentration was determined using
the Bradford assay (BioRad, Mississauga, ON, Canada) and 25 ug of total protein
_lysate was used for each sample in the assay. Thereafter, the assay was performed
according to the manufacturer’s protocol, using the colorimetric, pNA substrate
provided. Absorbance readings were obtained using a pQuant microtitre plate
reader (Molecular Devices, Sunnyvale CA, USA), with readings taken every 10
minutes for a total of 120 minutes; the assay plate was held at 37°C between
readings. Calculation of enzymatic activity was done using the slope of the linear
portion of the time course.
2.3.6 Western blotting
To assess protein expression in ICR and C57BI/6 placentae, two to three
placentae from each dam were placed in PBS containing a Complete™ protease
63
inhibitor tablet (Roche, Laval, QC, Canada), dissolved according to manufacturer's
instructions. Pooled placentae were weighed, placed on ice and 1 x SDS sample
buffer (62.5 mM Tris-HCl, pH 6.8; 2% w/v SDS; 10% glycerol; 50 mM DTT; and
0.01% w/v bromophenol blue) was added at a ratio of 1 mg tissue: 9 uL sample
buffer. The tissue was vigorously homogenized over ice, followed by several
passages through an 18 % gauge needle and a 23 % gauge needle fitted to a
syringe, in order to more thoroughly homogenize the tissue and shear the DNA. If
not used immediately, samples were stored at -80°C. Individual d15.5 Bax WT
(n=5) or KO placentae (n=5) were similarly treated, except decidual tissue was
removed (Figure 2.10a) prior to weighing and homogenization. Lastly, samples of
labyrinthine tissue from WT, KO or heterozygous (Het) d14.5 and d18.5 placentae
were “punched out” (Figure 2.12b) using a 2-mm Keyes tissue punch (Roboz
Surgical Instruments, Gaithersburg, MD, USA).
Standard denaturing acrylamide gels of varying concentrations and
electrophoresis buffer were prepared according to instructions provided by the
manufacturer of the electrophoresis apparatus (Novex). For each lane, 8.5 UL of
sample was mixed with 8.5 pL of 1 x SDS buffer supplemented with B-
mercaptoethanol (Sigma) at a ratio of 49:1. Samples were then held at 100°C for 3
minutes, allowed to cool and centrifuged briefly; 15 pL of sample was loaded per
lane. Proteins were transferred to 0.2 um Biodyne nitrocellulose (VWR) and blots
were stained with Ponceau S (Sigma) and then blocked for 1 hour with 5% skim milk
in Tris-buffered saline (TBS) with 0.1% Tween 20 (TBST) for 1 hour. The following
primary antibodies were used: anti-caspase-3 (1:500; Cell Signalling); anti-Bax NT
64
(1:500); anti-placental lactogen | (1:100; Chemicon); anti-placental lactogen II
(1:100; Chemicon); anti-cleaved Parp-1 (1:500, Cell Signalling); and anti-PECAM-1
(1:100; Santa Cruz Biotechnology, Santa Cruz, CA, USA). Blots were stripped and
reprobed with anti-B-actin antibody (1:400, Santa Cruz) to correct for protein loading.
Each antibody was diluted in 3% skim milk in TBS and membranes were held
overnight at 4°C, with gentle shaking. Blots were then washed 4 x 5 minutes with
TBST and probed with a solution of 1:1000 of appropriate secondary antibody
conjugated with alkaline phosphatase (AP; BioRad) in 3% skim milk in TBS. After 4
X 5-minute washes with TBST, membranes were incubated with ECF substrate (GE
Healthcare) and scanned on a STORM imager (Molecular Devices). Densitometric
analyses were done using ImageQuant® software.
2.3.7 Statistical analysis
ICR and C57BI/6 placental cell death rates and protein expression levels over
gestation within one strain and between the two strains were analyzed by one-way
and two-way ANOVAs, respectively. Cell death rates and protein expression levels
for Bax WT versus KO placentae were analyzed by two-way ANOVA. Post-hoc
comparisons of means were analyzed using the Tukey-Kramer test. All other data
were analyzed by Student’s t-test. Statistical software used was SPSS® (Version
13) and data were considered statistically significant if p < 0.05.
65
2.4 Results
2.4.1 ICR and C57BV/6 conceptuses and decidua display similar numbers and patterns of TUNEL positivity at d7.5
At d7.5, the regions demonstrating the greatest number of TUNEL-positive
cells were the mesometrial and anti-mesometrial decidual cells directly adjacent to
the EPC and distal endoderm, respectively. The anti-mesometrial decidua in both
strains studied exhibited significantly higher rates of cell death compared with that
seen in the mesometrial decidua (Figure 2.2a). Additionally, the uterine cavity often
contained TUNEL-positive, detached cells and debris, including free, fragmented
DNA (Figure 2.2b). The EPC exhibited infrequent cell death, with no discernible
evidence of an organized pattern. The allantois was likewise observed to have a low
number of dead cells; however, the majority of TUNEL-positive cells were located at
the tip of this structure. A low percentage of TUNEL-positive TGCs (Figure 2.3a)
appeared sporadically around the EPC and the extraembryonic endoderm
(surrounding the embryo), with no evident pattern. However, a greater number of
primary TGCs demonstrated condensing nuclei and morphologically appeared to be
dying, but were TUNEL-negative (Figure 2.3b). Moreover, at d7.5 for both mouse
strains, there was a greater percentage of TUNEL-negative, condensing primary
TGC, compared with the characteristic, TUNEL-positive cells typically observed in
mid- to late-gestation. Lastly, several primary TGCs contained TUNEL-positive cell
corpses that had been phagocytosed (Figure 2.4). Comparisons between the data
obtained from ICR and C57B//6 placentae at d7.5 yielded no significant differences
in TUNEL positivity in the various cell types and regions studied (i.e. mesometrial
66
Figure 2.2 Cell death patterns in d7.5 ICR and C57BI/6 conceptuses. A. Graph
depicts the number of TUNEL-positive cells per 100 um? of tissue. B.
Photomicrograph demonstrating the uterine cavity of a d7.5 ICR conceptus,
containing TUNEL-positive debris and nuclei. Mesometrial and anti-mesometrial
poles of conceptus are indicated. C. Left panel consists of low- and high-
magnification photomicrographs of d7.5 ICR EPC, with arrow indicating TUNEL-
positive trophoblast cell within EPC. Right panel consists of low- and high-
magnification photomicrographs of d7.5 embryo, surrounding primary TGCs and
anti-mesometrial decidua. Filled arrowheads indicate TUNEL-positive primary TGC
healthy primary TGC nuclei. Bars represent average values + SE, with white and
black bars denoting TUNEL-positivity in ICR placentate (n=8) and C57B//6 placentae
(n=6), respectively. Values of significant statistical difference between different
tissue regions are shown with corresponding p value (Tukey-Kramer post-hoc test).
67
A. TUNEL-positive cells in d7.5 conceptuses
p=0.0013
0.9; p=0.0019 | @ 0.8 4
g 0.7 J O-Icr ot 06 4 @ c57BI6
Bs 05 YO 10 7 °
aS o4. in 6 > 2 0.3 -
E 0.2 4 0.1 4
0 n=8 n=8 n=8
Mesometrial . Anti-mesometrial EPC
decidua decidua
B.
TUNEL-positive debris
and nuclei
‘| anti-mesometrial
pole
mesometrial
d7.5 ICR ectoplacental cone d7.5. ICR primary TGCs
Figure 2.2
68
and anti-mesometrial decidua, EPC, allantois and primary TGCs). Note that positive
(sections pre-incubated with DNase | enzyme) and negative (sections incubated
without Tdt enzyme) controls for TUNEL-staining at varying gestational timepoints
yielded high levels and absent TUNEL-positivity, respectively
2.4.2 Murine placentae exhibit organized cell death patterns over gestation; however, differences in the number of TUNEL-positive cells exist between the two strains
By d10.5, all major regions of the mouse placenta are evident. Herein, the
data will be reported for each region at the gestational timepoints examined.
Trophoblast giant cells: d10.5 — d18.5
Several different morphological features of TGC death emerged over
gestation: (1) TGC with condensing, TUNEL-positive nuclei; (2) TGC with swollen,
TUNEL-positive nuclei and TUNEL-positive cytoplasm; (3) TGC with TUNEL-
negative nuclei, but strong chromatin condensation and cell shrinkage; and, (4)
healthy TGC containing phagocytosed, TUNEL-positive cell debris and/or nuclei. At
all timepoints examined, for both ICR and C57BI/6 placentae, these features of
TUNEL-positivity in TGCs were evident. Towards the end of gestation, there were
increased rates of both types (1 and 2) of TUNEL-positive TGC in both strains
examined; however, from d15.5 — d18.5, this rate was significantly higher in C57BI/6,
compared with ICR placentae (Figure 2.3a). At d10.5, the percent cell death within
the four different groups of TGC appeared approximately equal (Figures 2.3, 2.4);
69
however, this pattern changed at d13.5 and continued until term, with the majority of
TGC in both strains exhibiting TUNEL-positive TGC nuclei (type 1 and 2). Lastly,
the sites of dead/dying TGCs — whether TUNEL-positive or condensing — were
largely confined to the lateral aspects of the placentae, with TGCs in and around the
midline of both ICR and C57B\/6 placentae typically appearing healthy. The percent
of TGCs containing TUNEL-positive cell corpses remained relatively consistent over
time, with a small, but significant decrease observed over gestation (Figure 2.4). In
addition, these cells were intermittently scattered throughout the TGC border, with
no discernible pattern evident, except for a tendency towards being at the maternal
edge of the maternal-fetal interface.
Chorionic Plate: d10.5 —d18.5
TUNEL-positive cells were observed in the chorionic plate at all timepoints,
with increasing numbers of labeled cells as gestation progressed (Figure 2.5a).
Labelled CP cells were examined at high magnification and the pattern of staining
appeared confined to the nuclei, with little to no free, labeled DNA within the
cytoplasm. The majority of cell death was located sporadically throughout the CP,
with some clustering of TUNEL-positive cells around smaller blood vessels. The
cells around the umbilical veins and arteries typically appeared unlabelled and did
not exhibit morphological signs of apoptosis at all gestational timepoints examined.
The CP of C57BI/6 placentae appeared to contain greater numbers of TUNEL-
positive cells compared with the CP of ICR placentae; however, this trend was
statistically significant only at mid-gestation (Figure 2.5a).
70
Figure 2.3 Trophoblast giant cell death patterns in ICR and C57BL/6 placentae
over gestation. Graphs depict the percentage of (A) TUNEL-positive or (B)
TUNEL-negative, condensing TGCs per placental section in ICR and C57BI/6
placentae over gestation. Accompanying photomicrographs in panel below
exemplify characteristic, TUNEL-positive (solid arrowhead) and condensing (arrows)
TGC nuclei in d15.5 ICR placentae; open arrowheads indicate healthy TGC nuclei
and asterisks (*) indicate maternal blood sinuses. Bars represent average values +
SE, with white and black bars denoting ICR placentate (ng7.5=8, nato.5=8; for all other
timepoints, n=9) and C57BI/6 placentae (nqg7.5=6, Na1o.5=8; for all other timepoints,
n=9), respectively. Within the same strain over gestation, means with the same
letter are not significantly different from each other (Tukey-Kramer test, p<0.05).
Values of significant statistical difference between ICR and C57BI/6 placentae are
shown with corresponding p value (Tukey-Kramer test).
71
A. TUNEL-positive Trophoblast Giant Cells
10 O ICR
8 @ C57BI/6
6 b,c b’
a,b a’ , 4 ; a a
: (ice 0 d7.5 d10.5 d13.5 d15.5 d17.5 d18.5
Percentage
of TUNEL-positive
TGC
per
sect
ion
(%)
TUNEL-negative, Condensing Trophoblast Giant Cells
10 C] ICR
mM C57BI/6
laaaa d10.5 d13.5 d15.5 d17.5 d18.5
Percentage
of condensing
TGC
per
sect
ion
(%)
d15.5 ICR placentae - trophoblast giant cells lining maternal venous sinuses
Figure 2.3
72
Figure 2.4 Percentage of trophoblast giant cells containing TUNEL-positive
corpses in ICR and C57BL/6 placentae over gestation. Graph depicts the
percentage of TGC containing TUNEL-positive corpses in ICR and C57BI/6
placentae over gestation. Accompanying photomicrograph below graph depicts a
TGC (cell border indicated by dashed line) containing two TUNEL-positive corpses
(arrowheads) within the cytoplasm. An adjacent, healthy TGC, without cell corpses
is indicated by the open arrowhead. Bars represent average values + SE, with white
and black bars denoting ICR placentate (ng7.5=8, Nuio.5=8; for all other timepoints,
n=9) and C57BI/6 placentae (Nng7.5s=6, Ng10.5=8; for all other timepoints, n=9),
respectively. Within the same strain over gestation, means with the same letter are
not significantly different from each other (Tukey-Kramer test, p<0.05).
Perc
enta
ge
of TGC
cont
aini
ng TUNEL-
positive co
rpse
s per
sect
ion
(%)
Trophoblast Giant Cells containing TUNEL- positive Corpses
73
9] a 8 74 a
74 ClIcr 6 - ™@ C57BI/6
3 b ob b
4) b b 3 5 Cc c
c Cc 2) d
‘ i: 0 2 0 ro 0 10 0 ™ Oo oO LO ™ eo
° o 5 o oO o
d15.5 ICR placenta: trophoblast giant cell containing cell corpses
Figure 2.4
74
Labyrinth: d10.5 — d18.5
For both ICR and C57BI/6 placentae, the cells of the labyrinth exhibited a
sporadic pattern of death until d13.5, as TUNEL-positive cells were randomly
scattered throughout this region. The number of labeled cells per 100 um? at d10.5
was similar for both strains examined (Figure 2.5b); however, at d13.5, the number
of dead cells in C57BI/6 labyrinth was elevated. At d15.5, in addition to the
previously observed sporadic cell death, a pattern of TUNEL-positive cells clustered
around the vasculature (Figure 2.5b) became evident in both ICR and C57BI/6
placentae; however, there were a greater number of these clusters in C57BI/6,
compared with ICR placentae, resulting in a significantly greater number of TUNEL-
positive cells per 100 ym? labyrinth in C57BI/6 placentae (Figure 2.5b). The majority
of these dead and/or dying cells appeared to be fetal endothelial cells and
trophoblast cells lining the maternal sinusoids; however, occasional ST nuclei were
also observed to be TUNEL-positive. As gestation progressed toward term, the
number of TUNEL-positive cells located sporadically within the labyrinth diminished
for both ICR and C57BI/6 placentae. Conversely, the number of cells dying in
groups around the vessels increased for ICR labyrinth towards d18.5, while this
pattern appeared unchanged in C57BI/6 placentae. The net result of these changing
patterns in TUNEL positivity was that there was no change with gestation in the
number of dead cells within the labyrinth in ICR placentae and a trend towards
decreased numbers of dead cells in the labyrinth in C57BI/6 placentae; however,
C57B\/6 labyrinth still demonstrated significantly greater numbers of TUNEL-
75
Figure 2.5 TUNEL patterns in ICR and C57BI/6 chorionic plate and labyrinth
over gestation. A. Graph depicts the number of TUNEL-positive nuclei per 100
um? of CP over gestation. Photomicrograph in right panel is a representative picture
of typical TUNEL-positive nuclei in d15.5 CP; arrowheads indicate TUNEL-positive
CP nuclei. B. Graph depicts the number of TUNEL-positive nuclei per 100 ym? of
labyrinth over gestation. Photomicrograph in right panel represents sporadic TUNEL
positivity seen in d15.5 labyrinth; photomicrograph in lower right panel depicts typical
cell death patterns seen along the labyrinthine vessels. Arrowheads indicate
TUNEL-positive labyrinth nuclei and arrows indicating nucleated fetal red blood cells
within dying/dead vessel. C. Graph depicts the number of TUNEL-positive nuclei
per 100 pm? of spongiotrophoblast within the labyrinth layer; accompanying
photomicrograph depicts characteristic TUNEL patterns observed in trophoblast
cells of this tissue. Dotted lines indicate the border between the labyrinth and the
spongiotrophoblast surrounding the maternal blood canal, indicated by asterisk (*);
empty arrowheads indicate TUNEL-positive nuclei in trophoblast cells encircling the
maternal blood. White bars represent average values for ICR placentae (n = 9 for all
timepoints except ng1o.s = 8) and black bars represent average values for C57BI/6
placentae (n = 9 for all timepoints except ngio.s =8) + standard error (SE). Within the
same strain over gestation, means with the same letter are not significantly different
from each other (Tukey-Kramer test, p<0.05). Values of significant statistical
difference between ICR and C57BI//6 placentae are shown with corresponding p
value (Tukey-Kramer test).
TUNEL-positive cells in Chorionic Plate
=0.04 . 1.6; nc b’
gE 144 =0.002 ; b’ — cick = § b b 5 & 1) mcs7Bve Se 1.04 85 os $3 a’ ae 06: 75 94] Zo Ee “— 4
d10.5 d13.5 d15.5 017.5 d18.5
TUNEL-positive cetls in Labyrinth
1.2 p=0.033 ~ TI ICR SIN
3 E 1.0 @ C57BI/6 by P=0.0032 2
82 08 » .p=0.0002
23 b b’ 82396 p=0.006 ge b’ ge 04 F ,
=
Woz) ag ae P = med
aa 0 dio05 d13.5 d15.5 d17.5 d18.5
TUNEL-positive Spongiotrophoblast Cells in Labyrinth
he Qa
a —
oe 1.8 Olicr p=0.019 1.6 Mi C57BI/6 p=0.007
#TUN
EL-p
osit
ive
cells
per
100 um
within La
byri
nth
(#cells/100
um
p=0.02
'
di3.5 d15.5 d17.5 di8.5
76
d15.5 C57BV/6 labyrinth - sporadic and
clustered death in upper and lower
panels, respectively
traversing through labyrinth, with encircling spongiotrophoblast cells
Figure 2.5
77
-positive cells at term, when compared with age-matched ICR labyrinth (Figure
2.5b). TUNEL-positive labyrinthine cells from both strains of placentae were
examined under high magnification for labeling patterns within the cell. Typically,
TUNEL staining was confined to the nuclei for those cells dying sporadically within
the labyrinth of both ICR and C57B\/6 placentae; little to no labeling of free DNA
within the cytoplasm was observed. For those cells clustered around the
vasculature of the labyrinth and exhibiting positive TUNEL positivity, labeled DNA
was observed both in the nuclei and cytoplasm of dying cells (Figure 2.5b).
Periodically, labeled cellular debris and free DNA were identified in both fetal vessels
and maternal blood spaces within the labyrinth.
As gestation progressed from d12.5 to term, SpT tissue appeared insinuated
within the labyrinth region of the mouse placenta, often completely differentiating to
GlyT by d18.5. At d13.5, both ICR and C57BI/6 placentae demonstrated similar,
comparatively high numbers of TUNEL-positive cells within these SpT pockets.
From d15.5 — d18.5, there was a significantly greater number of dead cells in these
regions in C57BI/6, compared with ICR labyrinth (Figure 2.5c). Although occasional
SpT/GlyT cells within the labyrinth were TUNEL-positive and sporadically placed, the
majority of labeled trophoblasts were directly adjacent to large, maternal blood
canals traversing through the labyrinth (Figure 2.5c).
Junctional zone: d10.5 — d18.5
The cells of the junctional zone (JZ) consist of SoT and GlyT. Cells of the JZ
in the placenta of both ICR and C57BI/6 mice exhibited a trend towards increased
numbers of TUNEL-positive cells over gestation (Figure 2.6). At earlier
78
developmental timepoints, cell death within the JZ was sporadic; however, at d15.5
in ICR placentae, SpT cells within the JZ, bordering on the labyrinth, began to exhibit
small clusters of TUNEL-positive cells (less than ten positive cells per group) which
was was apparent through to d18.5. Furthermore, GlyT cells of the JZ in d15.5 ICR
placentae similarly demonstrated focal regions of collective cell elimination at the
maternal-fetal interface (Figure 2.6); however, these focal regions were much
smaller in size (typically less than ten TUNEL-positive nuclei). These patterns of
grouped, TUNEL-positive cells at the maternal-fetal interface and the labyrinth-JZ
border were not evident in C57BV/6 placentae until d17.5 and d18.5,
respectively; indeed, the pattern of cell death in these regions appeared sporadic at
these timepoints. At high magnification, the labeling in trophoblast cells of the JZ
was typically confined to the nuclei; however, occasional TUNEL-positive cells were
observed to have staining within the cytoplasm, especially in regions of clustered cell
death. At d10.5 and d18.5, the JZ of both ICR and C57BI/6 placentae exhibited
similar numbers and patterns of dead cells; however, at d13.5 — d17.5, cells of the
JZ in ICR placentae demonstrated significantly higher numbers of TUNEL-positive
cells, compared with C57BI/6 placentae.
The maternal compartment: d10.5 ~ d18.5
At mid-gestation, all TUNEL-positive cells were scattered within the maternal
compartment, and largely appeared to be cells of maternal origin (i.e.
decidual cells, uterine natural killer cells, glandular epithelium); the number of
TUNEL-positive cells in the maternal compartment increased over gestation, for both
79
Figure 2.6 TUNEL patterns in ICR and C57BV/6 junctional zone at specified
timepoints over gestation. Graph depicts the number of TUNEL-positive nuclei
per 100 um of junctional zone tissue over gestation. Accompanying
photomicrograph is a representative picture of typical TUNEL-positive nuclei in d15.5
junctional zone. Dotted line delineates the border between the labyrinth and the
spongiotrophoblast layer of the junctional zone; arrowheads indicate TUNEL-positive
spongiotrophoblast nuclei. White bars represent average values for ICR placentae
(n = 9 for all timepoints except ngio.s5 = 8) and black bars represent average values
for C57BI/6 placentae (n = 9 for all timepoints except ngios =8) + standard error
(SE). Within the same strain over gestation, means with the same letter are not
significantly different from each other (Tukey-Kramer test, p<0.05). Values of
significant statistical difference between ICR and C57BI/6 placentae are shown with
corresponding p value (Tukey-Kramer test).
#TUN
EL-p
osit
ive
cells
per
190
um2
of JZ (#
cell
s/10
0 um
*)
02 92
090
90 oO
bh
Oo bk
UT OD
i L
i L
}
80
TUNEL-positive cells in Junctional Zone
p=0.011
p=0.033 b
b
p=0.0008 a o) ©: a
~~»
ied)
b’
o
PP
wh
I
d105 d13.5 di5.5 d17.5 d18.5
d15.51C
Figure 2.6
81
mouse strains studied (Figure 2.7a). In addition, there was elevated sporadic cell
death within the maternal compartment of C57BI/6 placentae, compared with ICR
placentae. At d15.5, focal regions of TUNEL positivity were observed in the
maternal compartment, located closely to the fetal-maternal interface (Figure 2.7b,c).
Additionally, clusters of TUNEL-positive cells often appeared to encase the large,
maternal arteries entering the JZ of the placenta and occasionally surrounded
maternal venous sinuses as well. The pattern and timing of this death varied
between the two mouse strains examined. For ICR placentae, the peak percent
area of clustered cell death within the maternal compartment was at d17.5, followed
by a dramatic decrease at d18.5 (Figure 2.7b). At this timepoint, these foci were
largely TUNEL-negative (only a faint brown stain was evident), and instead
appeared as masses of acellular tissue. In C57BI/6 placentae, a similar clustering of
dead/dying cells around the maternal blood canals was observed; however, the
percentage of TUNEL-positive lesions in the maternal compartment of C57BI/6
placentae was significantly lower than those in ICR placentae at all timepoints
examined (Figure 2.7b). Additionally, there was little to no evidence of TUNEL-
negative, acellular patches of tissue at the maternal-fetal interface — as seen in ICR
placentae — in C57BI/6 placentae at d18.5.
82
Figure 2.7 Maternal decidual cell death patterns in ICR and C57BL/6 placentae
at specified timepoints over gestation. A. Graph depicts the number of sporadic,
TUNEL-positive nuclei within maternal decidua of ICR and C57B//6 placentae over
gestation. Accompanying photomicrograph illustrates a region of maternal decidua
with sporadic, TUNEL-positive nuclei (arrowheads). B. Graph represents the
percentage of area in the maternal compartment that exhibits focal regions of
TUNEL-positivity for ICR and C57BV/6 placentae over gestation. Accompanying
photomicrograph depicts a focal region of TUNEL-positive nuclei within the maternal
compartment, with open arrowheads indicating healthy TGC in the TGC border. C.
Photomicrograph of maternal vessel (demarcated by dotted line) in decidua at
maternal-fetal interface, surrounded by foci of TUNEL-positive nuclei and acellular
tissue. Solid line represents one of the focal areas of TUNEL positivity. Asterisk (*)
represents a patch of acellular material. Bars represent average values + SE, with
white and black bars denoting TUNEL-positivity in ICR placentate (ng7.5=8, ngi9.5=8;
for all other timepoints, n=9) and C57Bl/6 placentae (ng7.5=6, Ngio.5=8; for all other
timepoints, n=9), respectively. Within the same strain over gestation, means with
the same letter are not significantly different from each other (Tukey-Kramer test,
p<0.05). Values of significant statistical difference between ICR and C57BI/6
placentae are shown with corresponding p value (Tukey-Kramer test).
#TUNEL-positive
cell
s pe
r 2
(#cells/100
ym
o
) of maternal_tissue
Oo
100
ym
83
Sporadic TUNEL-positive cells in Maternal
compartment
CIcR p=0.028
6 5 m CS57BI/6 A d’
2 4 ype
p=0.031 cd’ 1 p=0.017 = b
8 7 b’,c’ : b’
| aa’ oa a
44
0 d10.5 di3.5 d155. di7.5 d185
Focal regions of TUNEL-positivity
in Maternal Compartment
RBS os
d15.5 ICR placenta - sporadic cell death in maternal decidua
i.
focal cell d15.5 ICR placenta - death in maternal decidua
wn
s p<0.0001 8 2 oo 164 b
85 12 a = p=0.0033 z 8 p=0.0005 - ‘ere 8 4 a - "SC a
SoS £—
o 2
= i ke ae J
§ 0 o d15.5 d17.5 d18.5
C.
d17.5:ICR placenta - foci of TUNEL- positive nuclei and acellular
tissue surrounding maternal vessel at maternal-fetal interface
84
2.4.3 Caspase-3 expression and localization are similar for ICR and C57BI/6 placentae
Activation of caspase-3 is considered to be a hallmark feature of cell death by
apoptosis. Both ICR and C57B//6 placental lysates exhibited similar levels of
cleaved caspase-3, with peak expression at early- to mid-gestation, followed by a
gradual decrease over the remaining developmental timepoints (Figure 2.8a). Note
that sections incubated with secondary antibody only, exhibited no staining. In
addition, caspase-3 enzyme assays revealed significantly higher activity in fetal-
enriched, compared with maternal-enriched fractions of d15.5 placentae, for both
strains examined (Figure 2.8b). While both fetal-enriched and maternal-enriched
placental lysates of C57BI/6 origin displayed higher levels of caspase-3 activity than
ICR placentae, this difference did not reach statistical significance.
Immunohistochemical analysis using cleaved-caspase-3 antibody on d15.5 placental
sections resulted in patterns of reactivity that were comparable to those seen after
TUNEL (Figure 2.8d). Evaluation of cleaved Parp-1 by immunoblotting revealed a
gradual decline of this protein in ICR placentae over gestation; however, in C57BI/6
placentae, cleaved Parp-1 peaked at d11.5, followed by decreased levels until term
(Figure 2.8c). Moreover, the cleavage profile of Parp-1 consistently demonstrated a
lack of the classical 89-kDa fragment and instead, exhibited Parp-1 cleavage
products of approximately 75 and 52 kDa.
85
Figure 2.8 Caspase-3 expression and activity in ICR and C57BI/6 placentae are
similar over gestation. A. Graph demonstrates procaspase-3 cleavage in
placental lysates as a densitometric ratio of cleaved caspase-3:total caspase-3 over
gestation, after Western blotting. Accompanying picture below graph is a
representative immunoblot of placental lysates from the indicated timepoints, against
anti-caspase-3 and anti-B-actin antibodies. B. Graph demonstrates the differences
in caspase-3 activity between the fetal and maternal compartments for ICR and
C57BI/6 placentae at d15.5. C. Graph depicts production of cleaved Parp-1
fragment at 75 kDa over gestation and accompanying picture below is a
representative immunoblot of placental lysates against anti-cleaved-Parp-1 and anti-
B-actin antibodies. Parp-1 cleavage fragments at 75 and 52 kDa are indicated and
arrow represents the putative position of the 89-kDa fragment. D. Representative
photomicrographs of fetal labyrinth (left panel) and maternal compartmental
placental tissue (right panel) in d15.5 C57BV/6 placenta, after cleaved caspase-3
immunohistochemistry. Arrowheads indicate cells positive for cleaved caspase-3,
arrows indicate nucleated fetal red blood cells within positively stained labyrinthine
vessels and asterisks (*) demarcate maternal blood spaces. Bars represent average
values + SE and n=3 for both ICR and C57BI/6 placentae, except where indicated in
panel C. Values of significant statistical difference are shown with corresponding p
value (Tukey-Kramer test).
Acti
vity
(p
mol/
min)
fo
r 25
pg
> Cleaved Caspase-3 Profile
0.8
0.6
3 0.4
Dénsitometric
ratio
of cleaved
caspase-3:total
caspase-3
3 r 0 “we
86
O Cleaved Parp-1 (75 kDa) Profile
0.7 p=0.0017 O IcR
Gi ier mM C57BI6 Mm. cé7aVe
Dens
itom
etri
c ra
tio
of cl
eave
d Parp-1
(75
kDa)
-act
in
09.5. d105 11.5: 0135 d16.5 17.5 18.5 9.6 di15.° di55 = 18.5
dood B-actin
oS 5.6 2.949 BGO Qh” yor ge
w Cagpase-3 Enzyme Assay
=0.006 : =0,016 =
np
o 5
aN
placental
tysate
NS
net re
32-35 kDa Procaspase-3
17-19 kDa Cleaved caspase-3
a a
t+ 75 kDa Parp-1 cleavage wb 52 kDa fragments
aii a FS] P-actin
~ 9.5 = —-d11.5— -d15.5- +d18.5~
d15.5 Fetal Labyrinth 15.5 Maternal Compartment ICR
CS7BI/6
Ei Sa EEEaamme md
towards towards decidua SpT and
Oo
Fetal-enriched Maternal-enriched maternal chorionic plate GlyTcells
compartment
Figure 2.8
87
2.4.4 Bax localizes to TGCs and the labyrinth of murine placenta and Bax deficiency leads to reduced TGC death and intrauterine growth restriction
Bax is a pro-apoptotic, channel-forming protein that has been implicated in
the regulation of cell death in the human placenta [322, 323]. Western blot
assessment of Bax expression in placental lysates revealed that in the ICR strain,
Bax levels significantly peak at mid-gestation and decrease towards term (Figure
| 2.9a). Interestingly, Bax expression in C57BI/6 placental lysates appears to
precipitously dip at mid-gestation. At all timepoints examined, Bax expression was
significantly greater in ICR placentae compared with C57BI/6 placentae (Figure
2.9a). Localization of Bax protein was determined by immunofluorescence in d15.5
placenta and revealed positive staining maternal decidua (data not shown), labyrinth
and a subset of TGC; other placental cell subtypes did not exhibit Bax staining.
Since Bax expression was detected in a subset of TGCs (Figure 2.9b),
patterns of death in this cell type were assessed in Bax WT and KO placental
sections using TUNEL. This assay demonstrated a significantl decrease in the
number of TUNEL-positive TGCs in Bax KO, compared with WT placentae, at both
d15.5 and d18.5 (Figure 2.9c). In addition, a greater proportion of TUNEL-positive
Bax KO TGCs exhibited the morphological features of necrosis and/or autophagy, as
opposed to the largely apoptotic or aponecrotic death that was observed in the
majority of TUNEL-positive Bax WT TGCs. Moreover, Bax KO placentae at d15.5
and d18.5 displayed significantly greater numbers of TGC per section, compared
with WT placentae at the same timepoints (Figure 2.9d, e). Further to this, while
Bax WT placentae yielded a significant decrease in the total number of TGCs per
88
Figure 2.9 Bax deficiency in murine placentae leads to decreased TGC death
over gestation. A. Graphs depict Bax expression levels in ICR (n=3 for all
timepoints) and C57BV/6 (n=3 for all timepoints) placental lysates over gestation. B.
Anti-Bax immunofluorescence in d15.5 Bax WT placenta, demonstrating positive
reactivity in TGCs and lack of staining in Bax KO TGC. C. Graph indicating the
percentage of TUNEL-positive cells per section in Bax WT and KO placentae, at
d15.5 and d18.5. D. Graph representing the total number of giant cells per section
in Bax WT and KO placentae, at d15.5 and d18.5. E. Hematoxylin-stained placental
sections of d15.5 Bax WT and KO placentae. The TGC border between the
maternal decidua and the fetal junctional zone has been demarcated in orange,
indicating the greater number of TGCs in Bax-deficient placentae. Bars represent
average values + SE. Values of significant statistical difference between ICR and
C57B\/6 placentae, or between Bax WT and KO placentae are shown with the
corresponding p value (Tukey-Kramer test). Within the same strain over gestation,
means with the same letter are not significantly different from each other (Tukey-
Kramer test, p<0.05). Nuclei in immunofluorescence photomicrographs are red and
Bax reactivity is green.
89
A. - Bax Expression in Placental Lysates over Gestation
8 2 p=0.001 C0 cr, ne3 3 1.8 b o 1.6 M@ C5786, n=3 6 14 242 p=0.012
c o's pr0.005 — p<0.001 p=0.02 BY p=0.002 3 06 a, ie
gS 04 ; ; bod % 02 a’d’ a’, a a‘. | ; B 0 d O d9.5 d10.5 d115 d13.5 15.5 d17.5 d13.5
B.
d15.5 Bax WT d15.5 Bax KO
C. Giant cell counts after TUNEL D. Total giant cell count
Bax WT = YD p=0.002
3 °° 7=0,008 mBaxkO 200 2 25 2 g p=0.04 5 160
25 20 ° 2% g 120 g x 15 7)
© 8 410 8 80 Wl < 5 5 & 40 te tH
ES 0 0
d18.5 d15.5
d15.5 Bax WT d15.5 Bax KO 7 mate
Figure 2.9
90
section from d15.5 to d18.5, Bax KO placentae did not exhibit such a decline over
the latter part of gestation (Figure 2.9d). Lastly, immunoblotting and densitometric
analysis of fetal-enriched placental lysates revealed increased levels of placental
lactogen | (PL-I) and placental lactogen II (PL-II) — both of which are TGC secretory
products — in Bax-deficient tissue (Figure 2.10b).
While total caspase-3 levels were significantly up-regulated in Bax KO
compared with Bax WT placentae, the ratio of cleaved caspase-3:total caspase-3
did not differ between the genotypes (Figure 2.10c). To ascertain whether caspase-
3 activity was affected, the same immunoblots were stripped and probed with
antibodies against PTEN, FAK and p21, which are known caspase-3 substrates [93,
324, 325]. This yielded no difference in cleaved protein:total protein (Figure 2.11),
verifying that indeed, caspase-3 activity is unchanged in Bax-deficient placental
lysates. Interestingly, levels of the 75 kDa fragment of cleaved Parp-1 was
significantly higher in Bax KO, compared with WT placentae (Figure 2.10d), while
the level of the 52 kDa fragment of Parp-1 was not significantly different between the
two genotypes (data not shown).
Bax expression was also identified in the labyrinth, with immunoreactivity
localized localized to the fetal endothelium and either one or both of the ST layers.
This was absent in Bax-deficient cells, confirming the specificity of the antibody
(Figure 2.12a). Confirmation of Bax expression in the labyrinth was determined by
Western blotting of labyrinthine-enriched lysates. As shown in Figure 2.12b, Bax
protein was detected in the placental labyrinth of heterozygous fetuses from Bax-
deficient dams. This supports the idea that detectable Bax in the labyrinth was
91
Figure 2.10 Bax deficiency in murine placentae leads to altered expression
levels of placental hormones and cell death markers. A. Photomicrographs of
dissection of d15.5 placental tissue into fetal-enriched and maternal-enriched
fractions; tissue was subsequently used for Western blotting (Bax placentae) or
caspase-3 enzyme assays (ICR and C57BI/6 placentae). B. Expression patterns for
PL-I and PL-II in d15.5 fetal-enriched, Bax WT and KO placental lysates after
immunoblotting and densitometric analysis. C. Caspase-3 expression patterns in
d15.5 fetal-enriched, Bax WT and KO placental lysates, after immunoblotting and
densitometric analysis. D. Parp-1 cleavage profile of 75-kDa fragment in d15.5
fetal-enriched, Bax WT and KO placental lysates after immunoblotting and
densitometric analysis. Representative immunoblot bands for Bax WT and KO
placental lysates are depicted alongside corresponding graphs, with B-actin used as
a control for protein loading. Bars represent average values + SE. Values of
significant statistical difference between Bax WT and KO placentae are shown with
the corresponding p value (Tukey-Kramer test).
Transverse slice of d15.5 placenta ~1-2 mm thick
Dens
itom
etri
c ratio
of
cleaved
casp
ase-
3:to
tal
caspase-3
Densitometric
ratio
of PL
~1
or total
caspase-3:actin
92
Se Discarded or used for caspase-3 assays
Maternal-enriched
fraction
Fetal-enriched fraction
Western blotting and Densitometry
Placental Lactogen Expression
in-d15.5 Placentae
p=0.007
12 Bax WT
40 | @ Bax KO s
3 WT KO WT KO - SS mee
2 dn. . ‘Guanes come . . 5 Lt R-actin R-actin
PL-I PL-Il
Caspase-3 Expression in d15.5
Placentae
p=0.03 0.45
0.35 @ Bax KO 0.3 Pro-caspase-3
0.25 0.2 Cleaved
0.15 caspase-3 0.1
0,05 = ee 0 oo : fS-actin
Cleaved caspase-3: — Total caspase-3:
total caspase-3 actin
D. Cleaved Parp-1 (75 kDa) in d15.5 Placentae
3 G © 16 "p=0.04 os BE 12 WT_KO #0 " i ss SS a aa cleaved Parp-1 2n™ 0.8 5 —
ao
—Ea04
a Bax WT Bax KO
Figure 2.10
93
Figure 2.11 Cleavage levels of active caspase-3 cellular substrates are not
altered in Bax-deficient placentae. Graph depicts densitometric ratios of
cleaved:total protein in d15.5 placental lysates, for known cellular targets of active
caspase-3. Representative immunoblot bands for Bax WT and KO placental lysates
are depicted alongside corresponding graphs, with B-actin used as a control for
protein loading. Bars represent average values + SE.
Dens
itom
etri
c ra
tio
of cl
eave
d
protein:total
prot
ein
Cleaved:total
94
Cleavage Profiles of Caspase-3 Substrates in d15:5, fetal-enriched Placentae
Cleaved:total Cleaved:total
FAK p21 PTEN
FAK: WT KO 125 kDa Full-length
75 kDa i Cleaved
p21:
21 kDa Full-length
14kDa —=} Cleaved
PTEN:
60 kDa Full-length
30 kDa Cleaved
Figure 2.11
95
contributed by the fetus and not the mother. Lastly, expression levels of PECAM-1
(an endothelial cell marker) were decreased in fetal-enriched placental lysates from
Bax-deficient placentae, compared with wildtype placental lysates (Figure 2.13a).
To more closely examine the labyrinthine architecture, lectin histochemistry was
used to distinguish the fetal endothelium [326]. The labyrinthine vasculature of Bax-
deficient placentae (Figure 2.13b) appeared slightly disorganized, with a looseness
and dilatation of both the endothelium-lined fetal vessels and the cytotrophoblast-
lined maternal blood channels at the same gestational timepoint. Moreover, this
altered labyrinthine architecture appeared more profound at later gestational stages.
To determine whether the morphological defects seen in the labyrinth had an impact
on the fetus, placental and fetal weights were obtained after heterozygous matings.
This revealed that while no difference was seen in fetal or placental weight at d15.5,
Bax KO fetuses at d18.5 demonstrated a small, but significant decrease in weight,
compared with d18.5 Bax WT fetuses (Figure 2.13c); no difference was observed for
placental wet weights.
96
Figure 2.12 Bax is expressed in the murine labyrinth. A. Anti-Bax
immunofiuorescence in d15.5 Bax WT placenta, demonstrating positive reactivity in
labyrinthine cells and lack of reactivity in the labyrinth of Bax KO placenta. B.
Photomicrograph in the left panel displays the results of microdissection, after
“punching” out portions of labyrinth and trimming off SpT from a slice of d15.5
placenta. Immunoblot to the right demonstrates the banding pattern obtained after
probing labyrinth-enriched lysates with anti-Bax and anti-B-actin antibodies. The
gestational timepoints and the fetal and maternal genotypes of the labyrinthine
lysates in each lane are indicated above and below the blots, respectively. Nuclei in
immunofluorescence photomicrographs are red and Bax reactivity is green.
Asterisks (*) represent maternal blood spaces and (tf) represent fetal vessels.
97
d15.5 Bax WT Labyrinth
d15.5 Bax KO Labyrinth
B. Confirmation of Bax expression in the labyrinth by microdissection
and immunoblotting:
Bax expression due to fetal contribution
to labyrinth
[oT d14.5 di85 di4.5 d18.5 d14.5 d185
Labyrinty Spongiotrophoblast &
ee ee -~— Bax
Labyrinth (.
— {$-actin
Fetal genotype: WT WT Het Het KO KO Maternal genotype: Het WT KO KO KO KO
Figure 2.12
98
Figure 2.13 Bax deficiency leads to abnormal labyrinthine structure and
intrauterine growth restriction. A. Graph depicts PECAM-1 expression in fetal-
enriched, d15.5 Bax WT and KO placental lysates, relative to the levels of B-actin.
B. Photomicrographs depict d15.5 and d18.5 Bax WT and KO labyrinth, after
probing with Bandeiraea simplicifolia and counter-staining with hematoxylin. C.
Graph depicts the wet placental and fetal weights obtained at d15.5 and d18.5, after
heterozygous matings. Bars represent average values + SE and values of
significant statistical difference are shown with the corresponding p value (Student's
t-test).
Weight
(9)
99
A. PECAN-1 Expression in Fetal-enriched
Placentae
= (0.07 a vO 2s 0.06 a E 8 0.05 Su 0.04 * p=0.04 gg i = A A B-actin
By 0.02 o. & 0.01 L n=5
d15.5 Bax WT d15.5 Bax KO
Low magnification: 15.5 labyrinth d18.5 labyrinth To err Se name
Bax WT |
Bax KO
d15.5 Placental and Fetal Weights d18.5 Placental and Fetal Weights
Bax WT p=0.05
m Bax KO
3S = 2 a
=
Piacenta Fetus Placenta Fetus
From.n=8 dams From n=8 dams
Figure 2.13
100
2.5 Discussion
Several pathological conditions complicating human pregnancies such as
preeclampsia , intrauterine growth restriction (for reviews see [20, 177]) and
exposure to cigarette smoke, have been shown to have aberrant placental cell death
profiles [327]. Although normal, human placental cell death over gestation has been
well studied, a systematic search into the extent and patterns of cell death in the
mouse placenta has been unavailable until now. The existence of homologous cell
types and cellular behaviour between these two species highlights the use of the
mouse as a suitable model for study of human placentation. Thus, analysis of
murine placental cell death patterns and molecular pathways is crucial, as it can aid
the study and interpretation of various genetic models and pathological conditions.
As has been previously shown in the human placenta [328, 329], cell death
appears comparatively infrequently during early placental development in the
mouse, giving way to a greater number of, and more organized patterns of dying
cells towards the end of gestation (Figure 2.14). In addition, different modes of cell
death (i.e. apoptosis, autophagy, aponecrosis, necrosis) were observed in several
placental cell types at varying gestational timepoints. Thus, sporadic, as well as
organized patterns of cell death are evident in the mouse placenta over gestation.
Strikingly apparent were the pockets of cell death that emerged at d15.5 in
the maternal compartment, closely adjacent to the M-F interface. A number of these
TUNEL-positive foci clustered around the large, maternal blood canals, creating the
impression that such massive, systematic death may provide a clean, efficient
separation of the placenta from the uterine wall upon parturition. Concomitant with
101
this expansion of dying cells in the maternal compartment, was an increased number
of TUNEL-positive cells in the junctional zone, particularly in the SpT and GlyT cells
within the fetal compartment. We propose that these clustered regions of death
within the junctional zone provide a similar function as that death which is seen in
the maternal compartment: specifically, to permit a clean separation from the
uterine wall, thereby protecting the mother and fetus from blood loss during delivery.
The observed trend of decreased cell death within the maternal and fetal
compartments adjacent to the M-F interface in inbred, C57BI/6 placenta are
suggestive of developmental delay, when compared with the outbred ICR placenta.
As fetuses of C57BI/6 mice exhibit growth curves indicative of IUGR (personal
communications, S.L. Adamson; and [330)), it is therefore possible, that abnormal
rates of cell death in these two regions surrounding the M-F interface have not yet
received the appropriate cell death cues. However, investigations into the precise
timing of both copulation and parturition in these two strains, or direct quantification
of placental markers over gestation, would be needed to clarify whether the
observed patterns in cell death reflect issues with developmental timing in the
C57BI/6 placenta.
Programmed cell death has been shown to have an important role in
embryonic development, with an impact on shaping such organs as the heart, digits
and brain (reviewed in [331-333]); it has also been implicated as having a role in
human placental morphogenesis [111]. Throughout life, PCD also functions to
102
Figure 2.14 Schematic representation of cell death patterns over development
in the mouse placenta. Pictures reflect typical cell death patterns as revealed by
TUNEL, that were observed in transverse sections of ICR conceptuses and
placentae at the timepoints examined in this study.
103
Dead cells, debris and free, fragmented DNA in uterine cavity
TUNEL-positive cells in maternal decidua - mainly
|
_*——-—~ Occasional TUNEL-positive EPC at mesometrial and anti- So a
!
i |
Severai_.in distal tip of allantois mesometrial poles
Occasional dead primary TGC
Occasional in proximal and distal endoderm
Corpses within primary TGC
d10.5
Sporadic cell death in maternal decidua
Occasional TUNEL-positive TGC
—\-— Corpses within TGC
maternal decidua and
fetal glycogen cells =~ Sporadic cell death in labyrinth and
\ chorionic plate
spongiotrophoblast
labyrinth
Sporadic cell death in maternal decidua
TUNEL-positive secondary TGC (| @ OO
chorionic plate
GB trophoblast giant cells Sporadic spongiotrophoblast ceil death
GE | dead or dying —w cells
TUNEL-positive labyrinthine ceils along
vasculature Focal regions of TUNEL-positive maternal decidual and fetal spongiotrophablast/glycogen
cells starting to form - mainly around large maternal vessels
Spongiotrophoblast surrounding large
vessels within labyrinth starting to die
Greater number of TUNEL-positive chorionic plate cells
d18.5 Regions of acellular tissue embedded with small, sporadic, TUNEL-
positive nuclei
Focal regions of TUNEL-positive maternal decidual and fetal
spongiotrophoblast/glycagen cells
Clustered spongiotrophoblast cell
death now evident
Figure 2.14
104
promote neovascularization in nascent or newly-functioning tissues, or to allow for
vessel regression and occlusion, as seen in the postpartum uterus (reviewed in [334,
335]). During early- to mid-gestation, cell death in the murine labyrinth occurred
sporadically and was infrequently observed; however, as development proceeded
from d13.5, TUNEL-positive cells exhibited typical clustering along the labyrinthine
vessels, with a trend towards an increased number of foci at d15.5, which was
slightly reduced by d18.5. It is likely that this “peak and decline” of labyrinthine cell
death, which was observed in both strains of mice studied, is a reflection of the
massive amount of remodeling required to serve increasing fetal demand. Thus, at
day 15.5, labyrinthine cell death along the vasculature is elevated — when fetal
demand is still comparatively low — to prepare for the impending vascular volume
and surface area [336] that is required at d18.5, when fetal demand is at a
maximum. While specific cell types of the labyrinth undergoing death were at times
difficult to identify, the fact that they were cells lining the vasculature was suggested
by the proximity of the dying cells to the fetal or maternal red blood cells within the
regressing vessels. Moreover, immunohistochemistry using anti-active-caspase-3
antibody revealed similar staining patterns along the vasculature as those seen in
TUNEL. It is possible that the cells involved may be endothelial cells (ECs) directly
involved in angiogenesis, as these have been shown to be more susceptible to
apoptosis compared to quiescent ECs [337]. In fact, it has been proposed that
priming angiogenic endothelial cells towards the cell death pathway allows for a
certain degree of “vascular pruning” during neovascularization [338].
105
Strain differences in labyrinthine cell death and in SpT pockets within the
labyrinth were readily apparent at mid-gestation, with C57BI/6 placentae displaying
significantly greater numbers of TUNEL-positive cells. A possible explanation for
this may be a placental response to reduced fetal growth by upregulating vascular
remodeling, leading to increased cell death; however, an equally compelling
argument is that the enhanced labyrinthine death in C57BI/6 mice results in IUGR.
In addition, dysregulated cell death has been proposed to be a mitigating factor in
gestational diseases such as preeclampsia and IUGR. Recently, two independent
studies have demonstrated higher rates of apoptosis in placental villi complicated by
IUGR [839, 340]; Levy et al. [339] reported that this increase was not associated
with upregulation of Bax protein [339]. These data support the hypothesis of
putative IUGR in C57BI/6 fetuses, as placentae from these dams exhibited elevated
cell death rates and decreased Bax expression, compared with ICR placentae.
Examinations of Parp-1 cleavage profile provided a platform for speculation
into possible alternative pathways involved in cell death execution during
placentation. Immunoblotting of placental lysates obtained from both ICR and
C57BI/6 mice at different gestational timepoints yielded Parp-1 cleavage fragments
at ~75 and 52 kDa, but a complete absence of the canonical, 89-kDa fragment,
known to be a product resulting from caspase-3 cleavage in other somatic cells [66,
341]. Various lysis buffers, two different anti-cleaved-Parp-1 antibodies and
modifications in sample preparation for gel loading were used to test the veracity of
this result, but all immunoblots demonstrated identical Parp-1 cleavage profiles.
Cells undergoing necrotic death have been reported to exhibit a different Parp-1
106
cleavage profile, yielding two major bands at 89 and 50 kDa [342], with lysosomal
cathepsins implicated in the production of this altered Parp-1 cleavage profile [343].
However, cell death triggered by the lysosomal pathway is not always necrotic in
nature; emerging evidence has shown that certain signals induce cathepsin release
from lysosomes, leading to the activation of the apoptotic pathway (for review see
[344]). Additionally, calpain, which is a Ca**-dependent cysteine protease, has
likewise been shown to produce 70-kDa [345] and 40-kDa [346] Parp-1 cleavage
fragments. Moreover, calpain has been associated with apoptotic events in
numerous cell types, but particularly in neurons [345, 347] and leukocytes [348,
349]. Interestingly, while the Parp-1 cleavage profile in ICR placentae followed a
similar pattern to cleaved caspase-3, C57BI/6 placental lysates did not exhibit such
uniformity, suggesting that the increases observed in the latter tissue may be due to
the activation of different caspases or alternate cell death pathways. In contrast,
different Parp-1 cleavage profiles may indicate roles for calpain and/or cathepsins in
trophoblast differentiation, as both these proteases have been associated with
differentiation events in other tissues [350-352]. Finally, both cathepsins and
calpains have been implicated during the development of both human and murine
placentae [353-356].
While the impact of disrupting various Bcl-2 family members has been
previously studied in many tissues and cell types, the placenta was not included in
these analyses [321, 357]. As a role for Bax in human placentation was also
proposed [322, 323], we decided to explore the potential of a placental phenotype
caused by a deficiency in this proapoptotic Bcl-2 family member. Both Bax and Bak
107
remain cytosolic until activation by apoptotic signals, upon which these proteins
translocate to the mitochondria and form membrane-spanning, oligomeric pores, in
an as-yet, unresolved mechanism [34], facilitating the release of several apoptotic
factors. The final consequence of this action is the formation of the apoptosome
[42], which leads to activation of downstream caspases, having a variety of specific
cellular targets [30]. In this study, we report Bax expression profiles in ICR
placentae, that peak at midgestation and gradually decrease towards the end of
gestation; however, Bax expression in C57BI/6 placentae was greatly diminished
compared with that seen in ICR placentae. Immunohistochemical studies revealed
positive Bax staining in a subset of TGCs and in a subset of cells within the
labyrinth. Moreover, the study of Bax-deficient placentae revealed the functional
significance of Bax in these two cellular layers. Bax KO placentae obtained from
heterozygous crosses exhibited increased TGC numbers compared with placentae
from wildtype littermates, attributable to diminished death rates of this cell type.
Additionally, immunoblotting studies revealed higher levels of PL-I and PL-Il in Bax-
deficient placentae, likely reflecting elevated TGC numbers. Moreover, TGC in Bax
KO placentae demonstrated a greater tendency towards autophagic- and/or
necrotic-like death, possibly caused by activating alternate cell death pathways due
to the absence of Bax and/or caspase activation [74]; however, the exact nature of
this death will require further investigation. Interestingly, while total caspase-3
expression and the 75-kDa Parp-1 cleavage fragment were upregulated in d15.5
Bax KO placentae, levels of cleaved caspase-3 were similar between WT and KO
placentae. The significance behind these seemingly contradictory data remain
108
uncertain; however, future studies will involve elucidating the different molecular
pathways involved in murine placental cell death, and hopefully, the meaning of such
enigmatic results will be made more apparent. Examination of the Bax KO labyrinth
region revealed an altered architecture, with apparent dilatation of both the maternal
blood spaces and fetal vessels. This was accompanied by an overall loose
organization of the labyrinthine vasculature, which also exhibited reduced
expression levels of PECAM-1. Further to this, d18.5 Bax KO fetuses exhibited a
small but significant degree of IUGR compared with Bax WT littermates, which is
likely attributable to the observed labyrinthine defects.
Conclusions
In conclusion, cell death patterns during murine placental development
appear similar to those seen in human placentae, with an overall increase towards
the end of gestation. While it is evident that cell death is involved in shaping the
vasculature of the murine labyrinth, the molecular pathways functioning in this region
and in other regions of the mouse placenta, remain to be elucidated. Lastly, murine
placentae deficient in Bax exhibit reduced TGC death and an altered labyrinthine
architecture that likely contributes to the observed IUGR; however, further studies
involving tetraploid rescue experiments will be required to determine whether this
growth restriction can be improved by correcting placental insufficiency.
109
CHAPTER 3
EMBRYONIC LOSS DUE TO EXPOSURE TO POLYCYCLIC AROMATIC
HYDROCARBONS IS MEDIATED BY BAX
A version of this chapter is published in Apoptosis, 2006, Volume 11, Issue 8, pp. 1413-1425, (Detmar J., Rabaglino T., Taniuchi Y., Oh J., Acton B., Benito A., Nunez
G. and Jurisicova A.). Reprinted with kind permission from Springer Science and Business Media. © Springer Science and Business Media, 2006.CHAPTER 3: Embryonic loss due to exposure to polycyclic aromatic hydrocarbons is mediated by Bax
REFERENCE: Detmar J., Rabaglino T., Taniuchi Y., Oh J., Acton BM., Benito A., Nunez G. and Jurisicova A. (2006) Embryonic loss due to exposure to polycyclic aromatic hydrocarbons is mediated by Bax. Apoptosis 11:1413-1425.
110
3.1 Abstract
The high miscarriage rates observed in women smokers raises the possibility
that chemicals in cigarette smoke could be detrimental to embryo development.
Previous studies have established that polycyclic aromatic hydrocarbons (PAHs),
transactivate the aryl hydrocarbon receptor (AhR), leading to cell death. Herein we
show that PAH exposure results in murine embryo cell death, acting as a potential
mechanism underlying cigarette-smoking-induced pregnancy loss. Cell death was
preceded by increases in Bax levels, activation of caspase-3 and decreased litter
size. Chronic exposure of females to PAHs prior to conception impaired
development, resulting in a higher number of resorptions. This embryonic loss could
not be prevented by the disruption of Harakiri, but was diminished in embryos
lacking Bax. We conclude that exposure of early embryos to PAHs reduces the
allocation of cells to the embryonic and placental lineages by inducing apoptosis in a
Bax-dependent manner, thus compromising the developmental potential of exposed
embryos.
3.2 Introduction
Cigarette smoking has been associated with a number of female reproductive
problems, including compromised oocyte maturation, ovarian failure, sub-fecundity,
and infertility (reviewed in [358, 359]). Such negative effects have been documented
for both active and passive (i.e. second-hand) smoking, using both human
epidemiological and animal model studies (reviewed in [250, 251, 253, 360]). The
111
most serious outcomes of tested PAHs include impaired preimplantation embryo
development, early embryo mortality, stillbirths, intrauterine growth retardation and
reduced neonatal survival [252, 253, 361]. Several mechanisms have been
proposed to explain the mechanisms surrounding female sub-fertility and exposure
to tobacco smoke as it relates to ovarian [362, 363] or trophoblast [364, 365]
function, but there is still a dearth of information regarding the molecular
mechanisms involved.
Polycyclic aromatic hydrocarbons (PAHs), such as 7,12-
dimethylbenz(a)anthracene (DMBA) and benzo(a)pyrene (BaP) are released into the
environment in high quantities as a result of the incomplete combustion of fossil
fuels (wood and coal). PAHs may also be found in furnace gases and automobile
exhaust fumes; however, the primary route of human exposure to these compounds
is cigarette smoke. A recent study reported variable PAH levels amongst the
different brands of cigarettes, with the total amount of PAHs in mainstream smoke
ranging from 1 to 1.6 wg per cigarette [366].
There are several possible mechanisms by which PAHs can alter cell function
at the molecular level. These compounds are capable of directly altering DNA
structure by forming DNA adducts [281], resulting in DNA mutations in affected cells.
In addition, these compounds interact with aryl hydrocarbon receptor (AhR), a
member of the basic helix-loop-helix family of transcription factors. Both BaP and
DMBA elicit a biological response, at least in part, by activation of this receptor,
which is present in its unbound form in the cytoplasm [367]. Upon ligand binding,
the AhR translocates to the nucleus and heterodimerizes with the aryl hydrocarbon
112
nuclear translocator (ARNT). This heterodimeric transcription factor recognizes
specific DNA sequences called aryl hydrocarbon-, dioxin- or xenobiotic-response
elements (AHRE, DRE or XRE) and thus modulates the expression of target genes.
The expression of a variety of genes has been reported to be altered by ligand-
bound AhR, including xenobiotic metabolizing enzymes, growth factors and other
transcription factors [367, 368]. We have recently reported that both human and
murine ovaries respond to DMBA exposure by activating cell death within oocytes of
resting primordial follicles in an AnR-dependent manner [369]. While a large volume
of information exists regarding the toxic effects of PAHs, comparatively little is
known about the mechanisms by which these compounds exert their apoptotic
effect. The PAH/AhR complex activates the pro-apoptotic Bcl-2 family member Bax,
expression of which appears to be necessary for the induction of cell death in
oocytes, since animals lacking functional Bax are almost completely resistant to
PAH driven follicular atresia [8369, 370]. Additionally, Harakiri (Hrk), a pro-apoptotic,
BH3-only family member [371] was demonstrated to be up-regulated in Jurkat T
cells, after exposure to dioxin, a halogenated aromatic hydrocarbon with known AhR
agonist activity [372]. The purpose of the current study was to determine the
biological effects of PAHs and elucidate the mechanisms involved after in vitro and
in vivo exposure of murine preimplantation embryos to PAHs. The in vivo animal
model used (i.e. chronic, slow-release exposure of female mice to PAHs prior to
conception) was implemented to mimic the conditions that are frequently seen in
human populations, where many women stop smoking either before or during early
pregnancy, generally due to fetal health concerns [373, 374].
113
3.3 Materials and Methods
3.3.1 In vivo BaP and DMBA treatment
Hrk wildtype (WT), Hrk knockout (KO) or Bax heterozygous (Het) mice were
backcrossed for two generations onto an ICR background. Six-week-old ICR,
(Harlan, Indianapolis, IN, USA), Fz Hrk WT, Fe Hrk KO and Fe Bax Het virgin, female
mice were randomly separated into PAH-treated or vehicle-treated groups and
group-housed in separate cages. Animals were maintained in a controlled room with
a 12h light: 12 h dark cycle and allowed ad libitum access to rodent chow and water.
Separate preparations of 2 mg/mL BaP (Sigma, Oakville, ON, Canada) or DMBA
(Sigma) were dissolved in corn oil and subjected to waterbath sonication, to allow
full dissolution of the PAHs. These solutions were then mixed 1:1 for a final
concentration of 1 mg/mL DMBA and 1 mg/mL BaP, or 2 mg/mL PAHs. Animals
were given subcutaneous injections under the scruff of the neck, using a 26% gauge
needle. The following regimen was employed: one dose (2 mg/kg) per week for 3
weeks, then three weeks’ rest, followed by one dose per week for three weeks. The
final, cumulative dose for PAH-treated mice was 12 mg/kg; vehicle-treated animals
were given proportional injections of corn oil, according to body weight.
3.3.2 Mating and tissue collection
Four days after the last injection, female mice were mated with the
appropriate male stud (i.e. F2 Hrk WT males, Fo Hrk KO males, F2 Bax Het males, or
114
ICR males) of proven fertility. Gestational age was determined based on the
presence of a vaginal plug, with the morning of detection being embryonic day 0.5
(d0.5) of gestation. Plugged females were removed from the male and group-
housed in separate cages; it was ensured at all times, that PAH-treated and vehicle-
treated females were placed in different cages. Pregnant dams were euthanized by
cervical dislocation; ICR conceptuses were collected at various gestational
timepoints (d7.5, d9.5, d10.5 or d12.5), while Hrk WT, Hrk KO and Bax Het
conceptuses were collected only at d12.5. The pregnant uteri were placed in
phosphate-buffered saline (PBS) and the number of conceptuses and resorptions
was recorded. Uterine horns were torn open with forceps and conceptuses teased
out. Decidual tissue was removed from the embryonic membranes, which were
subsequently torn open to expose the embryo. Early embryos (d7.5) were assessed
for viability by morphology; later embryos (d9.5, d10.5 or d12.5) were assessed for
viability by morphology and the presence of a beating heart. Where required,
embryos were washed well with PBS and stored at -20°C for PCR genotyping. ICR
placentae with attached decidua were collected at d9.5, d10.5 and d12.5, and
placed in 10% phosphate-buffered formalin for 24 hours at 4°C for 24 hours, after
which the tissue was washed well with PBS and stored in 70% (v/v) ethanol until
paraffin embedding.
3.3.3 PCR Genotyping
Hrk Fz mice, Bax Fz mice and Bax embryos were genotyped by PCR as
previously described [357, 375] . ICR embryos collected at d9.5 or 10.5 were
115
digested overnight at 55°C in lysis buffer (60 mM KCI, 10 mM Tris-HCl, pH 8.3, 2
mM MgCl, 0.1 mg/mL gelatin, 0.45% Nonidet P40, 0.45% Tween 20) with
proteinase K (0.5 mg/mL final concentration). Proteinase K was heat-inactivated at
95°C for 10 minutes. PCR genotyping for the sex chromosomes was done in
separate reaction tubes, using primers for the Xist gene (X chromosome; forward
primer: 5° TTG CGG GAT TCG CCT TGA TT 3’; reverse primer: 5’ TGA GCA GCC
CTT AAA GCC AC 3’) and the Zfy gene (Y chromosome; forward primer: 5’ GAC
TAG ACA TGT CTT AAC ATC TGT CC 3’; reverse primer: 5’ CCT ATT GCA TGG
ACA GCA GCT TAT G 3’). X-chromosome PCR conditions were as follows: 2 mM
MgCle, 400 nM each primer and 200 nM dNTPs. Y-chromosome PCR conditions
were as follows: 2 mM MgCl, 800 nM each primer and 200 nM dNTPs. Cycling
conditions for both X and Y PCR were identical: 3 cycles of 95°C for 4 min., 52°C
for 1 min., 72°C for 1 min., followed by 32 cycles of 95°C for 1 min., 52°C for 1 min.
and 72°C for 1 min. Known male and female DNA obtained from ear punches were
used as controls. PCR reactions were run on a 2% gel and evaluated for the
presence of the 220 bp X band and the 200 bp Y band.
3.3.4 Collection of in vivo PAH-treated preimplantation embryos
PAH-treated and vehicle-treated ICR female mice were superovulated using 5
IU of pregnant mare serum gonadotropin (Sigma), followed 48 hours later by 5 IU of
human chorionic gonadotropin (Wyeth, St-Laurent, QC, Canada). The mice were
subsequently mated and the gestational timepoint was established as described
above. Embryos were retrieved at d3.5, by flushing the uterus with modified human
116
tubal fluid medium (Irvine Scientific, CA) then fixed in 4% paraformaldehyde, diluted
in PBS on microscope slides, air-dried and stored at 4°C until further use.
3.3.5 Collection and transfer of in vitro DMBA-treated embryos
Eight- to twelve-week old ICR female mice (Harlan) were superovulated using
the previously described protocol. Embryos were retrieved at the zygote stage
(d0.5) and placed in double-well dishes containing KSOM with amino acids
(Specialty Media, Phillipsburg, NJ, USA). In the afternoon of day 2.5, 8-cell embryos
were selected from a pool of cultured embryos and were randomly divided into
treatment groups (20-30 per group/per experiment). Embryos were cultured in 50 pL
microdrops under mineral oil (Specialty Media) supplemented with vehicle (DMSO)
diluted in the culture medium (0.002%) or DMBA (1 uM). DMBA stock was prepared
in DMSO as a 50 mM solution and diluted in medium prior to addition to a culture.
The synthetic AhR antagonist, o-naphthoflavone (ANF) was diluted in DMSO as
stock of 10 mM. The final dose used as an inhibitor of ANR was 2 uM, as previously
determined [369]. All compounds were purchased from Sigma. Embryos were
cultured in a humidified incubator at 37°C, 5% COs for forty-eight hours to assess
embryo development and evaluate other parameters associated with the activation
of cell death. Embryos that were not used for transfer were washed and fixed in 4%
paraformaldehyde, as described above.
To determine the developmental potential of treated embryos, blastocysts
exposed for 24 or 48 hours to vehicle or DMBA, were transferred into the uterine
117
horns of pseudopregnant females, mated with vasectomized males 2.5 days prior
transfer. Each female received 10 embryos (5 per uterine horn) in three
independent experiments with three females per group/experiment. Females were
allowed to deliver and the number of pups at birth was determined by visual
examination the morning after delivery, which was considered posinatal day 1
(PN1). Each pup was weighed on PN1 and PN21.
3.3.6 Analysis of cell number and cell death
Nuclear staining with the fluorochrome, 4,6-diamidino-2-phenylindole (DAPI,
Sigma) was used to analyze chromatin status. Embryos that had been treated with
vehicle or DMBA in vitro, then fixed and stored at 4°C, were stained in a 50 wg/mL
solution of DAPI in PBS for five minutes, washed with PBS, mounted with 30%
glycerol and viewed under a Zeiss Axioplan microscope. Assessment of mitosis and
cell death was based on DNA condensation, fragmentation and nuclear morphology
as previously described [376]. The cell death index (CDI) was calculated as the
percent of total cells that exhibited intense DAPI staining due to condensation of
chromatin, which in mammalian blastocysts is known to precede DNA fragmentation
[377]
Embryos that had been exposed to vehicle or BaP-DMBA mixture in vivo
were treated as above, but underwent further analysis using TUNEL assays; these
assays were performed as previously described [377].
118
3.3.7 Mitochondrial membrane potential analysis
JC-1 = (5,5’,6,6’-tetrachloro-1,1’,3,3’-tetraethylbenzimidazoyl | carbocyanine
iodide, DePsipher™ Kit TA700, R&D Systems Inc, Minneapolis, MN, USA) is a
lipophilic cationic dye which reflects the activity of mitochondrial membrane potential
and thus, is frequently used as an indicator of mitochondrial depolarization
associated with apoptosis [378]. Embryos were exposed to JC-1 and analyzed as
previously described [379]. Following staining, embryos were individually washed
and subsequently imaged on a deconvolution microscope (Olympus 1X70, Applied
Precision Inc., Issaquah, WA, USA), using fluorescein isothiocyanate (FITC) and
rhodamine isothiocyanate (RITC) filters. Optically sectioned images (each section
having a thickness of 5 um) were obtained, with a total of ten sections visualized for
each mouse embryo. Acquired images were analyzed using DeltaVision Software
(Applied Precision Inc., Issaquah, WA, USA), which allows for quantification of signal
intensity in each channel. The ratio of RITC (J-aggregate) to FITC (J-monomer)
staining was determined for all sections of the embryo, from which an average ratio
of J-aggregate to J-monomer staining for the entire embryo (n=13 for vehicle and
n=19 for DMBA-treated) was determined.
3.3.8 Single embryo caspase activity assay
This single cell fluorescent assay reflects predominantly the activity of
caspase-3 and -7, by trapping fluorochrome-conjugated caspase substrate (DEVD -
Asp-Glu-Val-Asp) within a cell. Caspase activity was assessed in exposed embryos
as previously described [321]. Briefly, embryos were cultured in the presence of
119
rhodamine-conjugated substrate (PhiPhiLux; Oncolmmunin Inc., College Park, MD)
for 3 hours, after 45 hours of exposure to vehicle or DMBA. Samples were
subsequently washed 3 times with PBS, fixed in 4% paraformaldehyde, transferred
onto slides and stained with DAPI as described above. This approach permitted
simultaneous analysis of chromatin status (diffuse or condensed), the distribution of
DNA and caspase-3-like activity. The total ratio of intensity of staining between
nuclear content and caspase-3 activity in several optical sections per embryo
(n=9/vehicle and n=10/DMBA) on rhodamine (red) and DAPI (blue) channels was
analyzed as described above for JC-1.
3.3.9 Expression of Bax and Hrk transcripts in exposed embryos
Gene expression was determined by a quantitative reverse transcription-
polymerase chain reaction followed by Southern dot blot analysis (QADB) assay
detailed previously [376, 380]. Briefly, cDNAs derived from three pools of five
blastocysts per treatment group (exposed to either DMBA or vehicle for 24 hours)
were amplified, dot blotted and analyzed by hybridization of dot blots with cDNA
probe radiolabeled by random-priming. Blots were exposed to a phospho-imager
cassette and the intensity of each dot was evaluated using ImageQuant Software.
The cDNA probe used contained part of the coding region and the 3'-untranslated
region of Bax and Hrk [376].
120
3.3.10 Immunocytochemical localization of Bax and AhR
Murine blastocysts were exposed to vehicle or DMBA for 24 hours, fixed for
10 minutes in 10% phosphate-buffered formalin, transferred to slides, air-dried and
stored at -20°C. Upon defrosting, slides were washed in PBS and microwave
antigen retrieval was performed in sodium citrate buffer (pDH=6.0) as previously
described [369]. Subsequently, slides were rinsed in PBS and blocked in 10%
normal goat serum in PBS with 0.05% Triton X. Affinity-purified rabbit anti-Bax P-19
(sc-526, Santa Cruz Technologies, Santa Cruz, CA, USA) or rabbit anti-AhR
(BioMol, Plymouth Meeting, PA, USA) polyclonal antibody diluted 1:100 in 5% goat
serum in PBS were applied to samples and incubated overnight at 4°C. Upon
further washing and incubation with diluted (1:200) secondary anti-rabbit biotinylated
antibody (Vector Laboratories, Burlingame, CA, USA), final labeling was performed
with streptavidin-Texas Red (Calbiochem, San Diego, CA, USA) and counterstained
with DAPI. The ratio of intensity of nuclear content to Bax immunostaining in several
optical sections per embryo (n=10/group) on DAPI and RITC channels was analyzed
using deconvolution microscopy, as described above.
3.3.11 Statistical analysis
Analysis of the differences in cell number, cell death, or mitotic rates between
treated and control groups was assessed by Kruskal-Wallis One Way Analysis of
Variance (ANOVA). Birth rates after transfer of exposed embryos were evaluated by
Chi-square analysis. All other statistical evaluations were done using the Student’s
121
t-test. All tests were performed using the SigmaStat statistical package (Version
1.0) and a p value < 0.05 was considered significant.
3.4 Results
3.4.1 Effect of DMBA on murine preimplantation embryos in vitro
Since previous epidemiological studies linked smoking with increased rate of
spontaneous abortions, we explored the possibility that a prototypical PAH, such as
DMBA, could function as a trigger for cell death, resulting in embryonic loss. We
used 8-cell preimplantation embryos, as this developmental stage is associated with
the second wave of embryonic genome activation, which is believed to be
responsible for the allocation of blastomeres to future cell lineages: the inner cell
mass (ICM) and the trophectoderm (TE). The dose of DMBA (1 1M) was
determined based on our previous experience with ovarian organ culture [369].
Moreover, pilot embryonic studies with this dose of DMBA did not exhibit non-
specific toxic effects, even when applied at earlier embryonic stages.
Addition of DMBA to the culture medium during the 48-hour period did not
interfere with the progression of embryos from the 8-cell stage to the expanded
blastocyst stage (d4.5). While embryos appeared slightly smaller, they contained a
distinct ICM and a defined blastocoele cavity. The total cell number, as well as the
mitotic index in the treated group, was slightly lower than in vehicle-treated embryos,
but the difference did not reach statistical significance. The only parameter
significantly (p = 0.012) affected by DMBA exposure was cell death, which was
increased in the treated embryos (Figure 3.1). Dead cells were localized to both the
122
ICM and the TE lineage and exhibited classical hallmarks of apoptosis, as indicated
by nuclear condensation, blebbing and fragmentation.
We further explored whether DMBA mediates its biological effect in the
murine blastocyst via the transcription factor, AnNR. Since previous reports
suggested embryonic expression of AhR in murine blastocyst by RT-PCR, we
performed immunocytochemistry using an anti-AhR antibody. Expression of AhR
protein was observed in both the ICM and TE, with exclusive cytoplasmic and
perinuciear localization of this protein. Upon exposure to DMBA for 24 hours,
occasional nuclear staining of AnR in a small number of cells was observed (Figure
3.2). Earlier time points (2, 4 and 6 hours) resulted in only cytoplasmic localization
of AhR. This suggests that DMBA, or its metabolites, function via nuclear
translocation and activation of AhR transcription. We further confirmed this
hypothesis by co-treatment of embryos with DMBA and ANF, a synthetic antagonist
of AhR, resulting in the rescue of DMBA-induced cell death (Figure 3.1). ANF alone
had no effect on embryo development, cell number, cell death or mitotic index.
3.4.2 Cellular and molecular pathways activated by DMBA
In order to determine whether DMBA activates similar cell death pathways in
the blastocyst as observed in primordial follicles of murine ovaries [369], we
assessed the expression of the pro-apoptotic Bcl-2 family member, Bax. Exposure
to DMBA for 24 hours significantly increased the levels of Hrk and Bax transcript in
blastocysts, when compared with vehicle-treated embryos (Figure 3.2). This was
followed in the next 24 hours by a 2-fold increase in Bax protein level/per nuclear
123
Figure 3.1 Exposure of murine preimplantation embryos to DMBA increases
the cell death index and AhR antagonist (ANF) precedes this effect. (A)
Representative micrographs showing the DAPI-stained nuclear morphology of
murine blastocysts incubated in vehicle 1 uM DMBA for 48 hours. Increased
numbers of cells with condensed and/or fragmented chromatin were observed
(arrows) in DMBA-exposed blastocysts. (B) The cell death index was significantly
increased (*p=0.0012, Student’s t-test) in DMBA-treated embryos, compared to
vehicle-treated embryos, after 48 hours. Depicted are the average values obtained
for vehicle-treated (white bars), DMBA-treated (black bars) embryos, DMBA, ANF
co-treated (dark grey bars), and ANF-treated (light grey bars) embryos + standard
error.
124
Vehicle
B. Effect of acute exposure of ANR agonist and antagonist on murine
preimplantation embryos in vitro
94 * p=0.012 8 aad
7: 0) Vehicle 2 @ 1M DMBA & a N m@ 1 uM DMBA + 2 uM ANF a en oe i 2 uM ANF L N ow iD Q 4- ul wt
Average “m
itot
ic an
d %dead
cell
Mitotic Index Cell Death Index
Figure 3.1
125
Figure 3.2 Cell death regulatory proteins are increased in DMBA-treated
murine blastocysts. Panels A-C are micrographs of representative embryos, with
cell-death-associated genes in red and nuclear staining in blue. As shown, the left
panel corresponds to vehicle-treated and the right panel to DMBA-treated embryos.
(A) Immunocytochemistry of arylhydrocarbon receptor (AhR) in murine embryos
exposed to vehicle or 1 uM DMBA for 48 hours. Representative nuclei from both
vehicle- and DMBA-treated embryos have been outlined in white to depict the
increased nuclear localization in embryos exposed to 1 uM DMBA for 48 hours. (B)
Immunocytochemistry of Bax protein in murine embryos exposed to vehicle or 1 uM
DMBA for 48 hours. (C) Trapping of caspase-3/7-cleaved substrate in vehicle-
treated or DMBA-treated murine blastocysts. (D) RT-PCR and dot-blotting of
pooled, murine embryos treated with 1 uwM DMBA for 24 hours, yielded significantly
higher Bax (**p=0.006, Student’s t-test) and Hrk ( p=0.05, Student's t-test)
transcripts, compared to pooled embryos treated with vehicle. (E) Estimation of total
Bax protein in vehicle (DMSO) or DMBA-exposed murine blastocysts. The ratio of
red/blue (protein expression/nuclear content) was determined in several optical
sections per embryo for a total of 10 embryos per group. Significantly increased Bax
(‘p=0.027) was observed in embryos held in 1 «M DMBA (black bars) for 48 hours,
compared to embryos exposed to vehicle (white bars) for the same length of time.
(F) Estimation of total caspase-3-like expression in vehicle- or DMBA-exposed
murine blastocysts. Values were obtained using a red/blue ratio as described above
for several optical sections per embryo, for a total of 10 embryos per group.
Significantly increased caspase-3/7 (‘p=0.047) was observed in embryos held in 1
126
uM DMBA for 48 hours, compared to embryos exposed to vehicle for the same
length of time. Bars represent average values + standard error.
127
; Increased Bax and Hrk expression in embryos Vehicle 1 uM DMBA D. exposed in vitro to DMBA for 24 hrs
5=0.05
~ nw oS
*p=0.006 O Vehicle
1 uM DMBA 80.
anti-AhR
a o
Densitometric
inte
nsit
y of
do
ts
after RT-PCR
and
biotting
ao
ae) Bax Hrk
E. Increased Bax expression in murine embryos exposed to DMBA in vitro
, | Tt p=0.027
anti-Bax : .
Vehicle 4M DMBA
‘on F . Increased caspase-3/7 activity in murine
embryos exposed to DMBA in vitro
=0.047 caspase-3/7 4 n=9 te rhodamine- I labelled : . substrate
Vehicle 1 uM DMBA
Figure 3.2
o
92 Bo
i o
2 ie =
bf it
ook,
oa
S —
Average
expr
essi
on
per
nuclear
content
per
cell
per
embryo
oO
° an
Qo - Q
NM
content
per
cell
pe
r embryo
So
Average expression
per
nuclear
128
content/embryo, as determined by quantitative analysis after immunostaining (Figure
3.2). These results are consistent with observations that a 48-hour exposure to
DMBA is needed for activation of cell death, as observed in neonatal murine ovaries
(Jurisicova and Matikainen, unpublished observation). Since Bax is known to
activate the mitochondrial pathway of apoptosis, we further assessed changes in the
mitochondrial membrane potential as indicated by a shift in the spectrum of
fluorescence of the cationic dye, JC-1. Due to the fact that changes of mitochondrial
membrane potential precede other hallmarks of apoptosis [381], we assessed the
ratio of JC-1 intensity after 43 hours of DMBA exposure. While we observed a
strong trend towards a decreased ratio of red/green fluorescence
(polarized/depolarized mitochondria) in the DMBA-treated group, this decrease did
not reach statistical significance (2.20 + 0.29 for vehicle and 1.63 + 0.18 for DMBA-
treated embryos). We attribute this lack of significance to the variability amongst
individual embryos caused by the transient nature of changes in mitochondrial
membrane potential.
Activation of effector caspases (caspase-3 and -7) was evaluated by
quantitative assessment of active caspases based on the cleavage of a rhodamine-
labeled substrate (DEVD), 48 hours after exposure to DMBA. We observed a
significant (~35%) increase (p = 0.0467) in the accumulation of caspase-mediated
fluorescence/per nuclear content in DMBA-treated blastocysts when compared with
vehicle-treated embryos (Figure 3.2). Thus, it appears that DMBA activates AhR,
resulting in increased levels of Bax protein, which in turn may activate cell death via
the mitochondrial pathway, resulting in the activation of caspases-3 or -7.
129
In order to determine the long-term developmental consequences of exposure
of murine embryos to DMBA, we transferred embryos exposed to vehicle or DMBA
for 24 hours (d3.5) or 48 hours (d4.5) into the uterine horns of pseudopregnant
females. As observed for cell death rates, only exposure to DMBA for 48 hours
caused a significant decrease (p = 0.021) in the number of pups born/embryos
transferred (30% [30 pups/90 embryos] in DMBA-exposed and 50% [45 pups/90
embryos] in vehicle-treated groups). Assessment of birth weight (PN1) as well as
weight at weaning (PN21) yielded no differences between vehicle- or DMBA-
exposed pups (Figure 3.3).
3.4.3 Maternal exposure to PAHs results in decreased pregnancy and increased resorption rates
Maternal cigarette smoking has been associated with increased rates of
spontaneous abortion and reduced fecundity. Additionally, female smokers are
increasingly apt to quit smoking prior to, or upon the onset of pregnancy. Our
murine model of slow-release injections of PAHs into virgin, female mice prior to
conception, mimics this human situation and our studies focused on the pregnancy
and resorption rates in PAH-exposed versus vehicle-exposed dams.
In order to determine the effects of maternal exposure to PAHs on murine
preimplantation embryo development, ICR females were exposed to BaP and DMBA
prior to conception, superovulated and mated to ICR males; embryos were retrieved
at d3.5 and assessed for cell death and mitotic indices. Six vehicle- and PAH-
130
A. PN1 Pup Weights 2.5
2
0 Vehicle
2 1.5) m PAH-exposed <=
> oO = 1 |
0.5
0 n=26 n=23
Male Female
B. PN21 Pup Weights 20
16 _ O Vehicle
2 424 m@ PAH-exposed
B oO = 8
4
0 n=23 n=23
Male Female
Figure 3.3 In vitro exposure of ICR preimplantation embryos to DMBA had no
effect on PN1 and PN21 weights. Graphs depict weights of male and female pups
at (A) PN1 and later at (B) PN21. Pups had been exposed to vehicle or DMBA in
vitro for 24 or 48 hours during the preimplantation stage and transferred to
pseudopregnant ICR females at d3.5 or d4.5. Bars reflect average values + SE.
131
treated dams were superovulated and successfully mated, however only 4 females
from each group yielded embryos useful for study. The number of obtained morula-
or blastocyst-stage embryos was decreased in the PAH-exposed females (n=74
from vehicle-exposed dams and n=54 from PAH-exposed dams). We observed a
reduction in the number of cells per embryo, resulting in ~20% loss of total number
of cells in embryos from PAH-exposed, compared with vehicle-exposed mothers.
This was accompanied by a trend towards increased cell death and mitotic indices in
embryos from PAH-exposed dams, as assessed by DNA morphology and TUNEL
staining (Figure 3.4).
Spontaneous pregnancy rates for PAH-exposed, ICR mice were reduced, as
only 60% (9 pregnant/15 plugged) of PAH-exposed, ICR females were pregnant
after excising the uterus 7, 9, 10, or 12 days after mating (determined by the
presence of a vaginal plug), compared with 100% (15 pregnant/15 plugged) of the
vehicle-exposed females. When PAH-treated females did conceive, there was a
significant increase in abnormal embryos, starting at approximately d7.5, leading to
early embryonic death determined by the greater number of resorptions and non-
viable embryos observed in d9.5 pregnant uteri of PAH-exposed females, compared
with vehicle-exposed females (Figure 3.5).
and
TUNEL-positive
(%)
Perc
enta
ge
of cells
in mitosis. dead
wn Le
be
Assessment of murine ICR preimplantation embryos after maternal exposure to PAHS
ned
n=67 C Vehicle ] Mf PAH-expased
n=47
% dead % TUNEL-
positive
3 per
embryo
bie
o
Average
total number
of cells
we
oS
132
Effect of maternal PAH exposure on ICR blastocyst cell number
Vehicle
§ PAH-exposed n=67
r ne5d
* p=0.0004
Vehicle PAH-exposed
Figure 3.4 Chronic maternal exposure to PAHs prior to conception results in
reduced cell number per blastocyst in d3.5, ICR preimplantation embryos. (A)
Trend towards decreased % mitotic and increased % dead (condensed chromatin,
blebbing, etc.) or TUNEL-positive cells in murine blastocysts obtained from dams
exposed to PAHs, prior to conception. (B) A significantly decreased number of cells
per embryo (*p=0.0004) was observed in blastocysts obtained from dams exposed
to PAHs, compared to dams exposed to vehicle. Bars from both (A) and (B) reflect
the average values + standard error for vehicle-treated dams (n = 4, white bars) and
PAH-treated dams (n = 4, black bars).
133
There are contradicting findings in human studies regarding the impact of
cigarette smoking and environmental pollution on the sex ratio of babies born at
term. Since our model of chronic PAH exposure in female ICR mice demonstrated
increased spontaneous abortion rates, we determined the sex genotype of live
embryos at d9.5-d10.5, for both vehicle- and PAH-exposed mothers. Tissue from
resorbing conceptuses was not available for PCR analysis, as the resorbing
embryos were far too damaged for extraction of good quality DNA. Seventy-four live
embryos from vehicle-treated dams yielded an almost equal proportion of both sexes
(Figure 3.5). Fifty-three live embryos from PAH-exposed dams yielded an average
proportion of 0.73 males per litter and 0.25 females per litter. Thus, while the
average proportion of either sex per litter did not differ in the vehicle-treated group,
the average proportion of males per litter was significantly different from the average
proportion of females per litter in PAH-exposed dams (Figure 3.5).
Since we observed that two cell death genes, Hrk and Bax, are upregulated in
embryos exposed to PAHs in vitro, we decided to establish if these genes were
necessary for the activation of death observed in PAH-exposed mothers. Hrk WT or
Hrk KO [375] mice — which are fertile and exhibit no overt phenotype — were
backcrossed for two generations onto an ICR background and exposed to the slow-
release PAH protocol, as described above. All PAH-treated females, regardless of
genotype, demonstrated a reduced number of embryos per litter, compared with
their vehicle-treated counterparts (Figure 3.6). Hrk KO and WT dams treated with
134
Figure 3.5 Chronic maternal exposure to PAHs prior to conception results in
an increased number of resorptions and a decreased number of viable
embryos, with a greater proportion of male embryos represented in the live
offspring. (A) A significantly decreased (*p<0.0001) number of morphologically
normal embryos and a significantly higher (**p=0.018) number of morphologically
abnormal embryos were obtained at d7.5 from ICR mothers exposed to PAHs (n=5
dams, black bars) compared to mothers exposed to vehicle (n=4 dams, white bars).
(B) A significantly decreased (‘p<0.0001) number of viable embryos and a
significantly higher (‘p=0.02) number of nonviable embryos were obtained at d9.5
from PAH-exposed mothers (n=6 dams) compared to vehicle-exposed mothers
(n=11 dams). Bars from graphs (A) and (B) reflect average values + standard error.
(C) ICR females chronically exposed to PAHs (n=8 dams, black bars) showed a
significantly different proportion of males, compared to females, per litter (“p=0.03).
ICR females exposed to vehicle (n=5 dams, white bars) had similar proportions of
males and females per litter. Bars reflect average proportions + standard error.
> Average
number
of viable
or
nonviable
embryos
per
litter
wD
Aver
age
number
of vi
able
, no
nvia
ble
or resorbing
embryos
per
litter
O Average
proportien
of ma
le
or female
embryos
per
litter
16 +
145
12 4
105
164
144
12 7
10 +
0.9
08
a7
0.6
0.5
4
a3
0.2
OA
135
Effect of maternal exposure to PAHS on
d7.5 ICR conceptuses
n=4
(] Vehicie
M PAH-exposed n=5
* p<0.0001 ** p=0.018
# embryos with # embryos with normal morphology abnormal morphology
Effect of maternal exposure to PAHS on
d9.5 ICR conceptuses
n=711
T Vehicle
n=6 W@ PAH-exposed
+ p<0.0001
tp=0.02
iw # viable embryos # nonviable # resorptions
Effect of PAHs on embryo sex in d9.5-d10.5
ICR mice
(1 Vehicle
i PAH-exposed n=
Males Females
Figure 3.5
136
Figure 3.6 Bax-deficient, but not Hrk-deficient, embryos are rescued from
resorption after chronic maternal exposure to PAHs, prior to conception. (A)
Hrk-deficient dams exposed to PAHs prior to conception demonstrated a similar
number of live embryos per litter, at d12.5, compared to PAH-exposed Hrk WT
dams. Bars represent average values + standard error for PAH-exposed WT (n=7)
and KO (n=9) dams and for vehicle-exposed WT (n=5) and KO (n=8) dams. (B)
Proportion of Bax wildtype plus heterozygous embryos (WT and Het) and KO
embryos, obtained by PCR genotyping, after exposure of Bax heterozygous females
to vehicle, or to PAHs, prior to conception. The proportion of Bax KO embryos per
litter in PAH-exposed mothers is significantly higher (**p=0.024) compared to the
proportion of Bax KO embryos from vehicle-exposed mothers. The proportion of
wildtype and heterozygous embryos per litter is significantly decreased (*p=0.024) in
PAH-treated mothers compared to vehicle-treated mothers. Bars represent the
average proportion of the genotypes for live, d12.5 embryos in vehicle-treated dams
(n=7, white bars) and PAH-treated dams (n=9, black bars).
137
Maternal exposure to PAHs in d12.5 Hrk WT or Hrk KO mice
p=0.007
n=
§ . 104
& 2 a- 5
Bz o5 2a eo = @ .ai
e 2. 2
o
e 0.9 5
B® os: -
G 07 4
o8 05; o 2 G44
ee 034 56 a 0.2 4
> on. zg
WT dams
p<0.001 O Vehicle M PAH-exposed
KO dams
# viable embryos
Maternal exposure to PAHs in d12.5 Bax heterozygous mice
n=65 () Vehicle, n=7 dams,
n=55 82 embryos
* p=0.024. @ PAH-exposed, n=9 dams,
85 embryos n=30 oy ** p=O.024
WT and Het KO
Genotype of viable embryos
Figure 3.6
138
PAHs demonstrated no significant difference in the number of embryos at d12.5.
Thus, disruption of Hrk is not sufficient to rescue the embryos from PAH-mediated
loss.
As Bax functions downstream of Hrk [382] and is also directly activated by
PAHs [369], this gene is more likely to have an effect on embryonic lethality.
However, as Bax KO females exhibit reduced fertility (J. Detmar and G. Perez,
unpublished observation) we used heterozygous mothers and assessed the
distribution of genotypes amongst surviving embryos at gestation day 12.5. The
genotypic proportions of offspring for heterozygous Bax females exposed to PAH
treatment differed significantly from the expected Mendelian ratios observed in
vehicle-exposed mothers, with a higher proportion of KO embryos, suggesting that
KO embryos are more resistant to embryonic loss triggered by PAHs (Figure 3.6).
3.5 Discussion
Several population-based human studies indicate that maternal cigarette
smoking carries serious reproductive hazards (reviewed in [383]). These include
delayed conception or infertility [258-260] as well as increased risk of spontaneous
abortion during natural or assisted conception [254-256]. While early pregnancy
loss has been previously linked to excessive activation of cell death [384, 385], the
molecular mechanisms involved in toxicant-mediated embryo demise are unclear.
Thus, we thought to explore this concept in an animal model, mimicking exposure to
a subset of chemicals found in cigarette smoke.
139
Animal studies using various types and sources of PAHs have shown that
exposure to these toxins can lead to decreased fetal survival [275, 277] or complete
postimplantation embryo loss [278]. Since these studies focussed on the
detrimental effects of PAH exposure in pregnant animals, we decided to test whether
female mice chronically exposed to PAHs prior to conception had a different
reproductive outcome. This model would be valuable in ascertaining what
pregnancy-related effects, if any, could be observed in animals treated with PAHs
prior to conception, a condition that is seen in human populations when women quit
smoking cigarettes before attempting to get pregnant. It was observed that ICR
females chronically exposed to a final, cumulative dose of 12 mg/kg of PAHs, prior
to conception, had a significantly decreased number of live embryos and a
significantly increased number of dead embryos at d9.5 of gestation. This translates
to a loss of approximately 35% of the litter in a PAH-exposed dam, compared with a
5% loss in control animals treated with vehicle. Additionally, PAH-exposed females
had a lower pregnancy rate compared with vehicle-treated females. Moreover, both
increased resorption rates and decreased pregnancy rates were still observed in
females up to 8 weeks after the final dose of BaP and DMBA (unpublished
observations, J. Detmar). Previous studies in rats have determined that after
intravenous BaP exposure, this chemical demonstrated a long half-life in a number
of different tissues [279] that can lead to persistence of DNA adducts in liver and
lung tissue [280]. Therefore, it would appear that PAH exposure prior to pregnancy
has long-lasting effects — at least with respect to spontaneous abortion and time to
140
conception — likely due to accumulation of these compounds and their metabolites in
various tissues.
DMBA has been extensively used as a prototypical ovotoxic compound [386]
with an unknown mode of action. We recently determined that DMBA/AhR
complexes activate the pro-apoptotic Bcl-2 family member, Bax. This pathway
appears to be necessary for the induction of cell death, since animals lacking
functional AhR or Bax are almost completely resistant to DMBA-driven follicular
atresia [369, 370]; however, dioxin — another potent AhR ligand — failed to activate
Bax and induce oocyte death in the ovary. This is due to minor changes in the
flanking nucleotide sequence adjacent to the tandem AHRE in the Bax promoter
[369]. This is also consistent with the observation that dioxin failed to compromise
preimplantation development or induce cell death in the murine blastocyst [387,
388], while DMBA proved capable of doing so in both oocytes and embryos (current
study). In both ovarian and embryo cultures, DMBA-mediated cell death required 48
hours of exposure and could be prevented by ANF, a synthetic inhibitor of AhR.
Ligand-engaged AhR resulted in the induction of Bax, followed by a slight change in
mitochondrial membrane potential and the activation of caspase-3. This was
observed in both the ICM and the TE, suggesting that the response of ovarian
follicles and cells of the early developing embryo utilize similar signalling pathways in
response to DMBA exposure. Moreover, DMBA exposure resulted in reduced live
birth rates, but only when cell death was induced at 48 hours, suggesting that cell
death contributes to either failed implantation or later embryo loss.
141
AhR expression in rabbit and mouse embryos has been previously described
[388, 389]. In the rabbit, blastocyst AnR expression is first localized to the polar
trophectoderm and eventually spreads to the embryoblast at later stages [390, 391].
Additionally, in vitro AnR antisense oligodeoxynucleotide experiments resulted in a
lower incidence of murine blastocyst formation, as well as a decreased mean
embryo cell number [389]. This suggests that AhR activity may be required for the
proper regulation of cell cycle progression. Our data indicate that excessive
activation of AhR by PAHs not only interferes with cell cycle, but also initiates
apoptosis. With the clear apoptotic effects of acute exposures to DMBA in embryos
observed in vitro, we proceeded to test the biological effects of chronic exposure to
PAHs in vivo. The use of more than one surrogate PAH and the injection of slow-
release doses over a period of nine weeks was designed to more closely parallel
PAH exposure found in human cigarette smokers. For these experiments, both
preimplantation and postimplantation embryos were examined, as preliminary in
vitro data suggested that PAHs had adverse effects on both stages in gestation.
While the mitotic and cell death indices did not reach statistical significance in
embryos exposed to PAHs in vivo, there was a trend towards increased cell death
and decreased mitosis in embryos from dams treated with PAHs, prior to
conception. Considering the transient nature of markers capable of detecting cell
death, in addition to the effective phagocytosis of cell debris by TE cells [392], even
these minor changes in cell fate resulted in a significant decrease in cell number in
PAH-exposed embryos.
142
Since embryonic resorption involves triggering the cell death cascade [393,
394], we tested whether mice with null deletions of Bax and Hrk — known
downstream targets of PAHs and dioxins, respectively — could rescue the resorption
phenotype seen in our model. Hrk is a pro-apoptotic, transcriptionally regulated,
BH3-only family member [375, 382]. It functions to induce cell death by binding to
pro-survival, Bcl-2 family members, thus de-activating their anti-apoptotic signals
and priming the cell for death [15]. Bax operates downstream of Hrk, forming pores
in the outer mitochondrial membrane and allowing release of apoptotic factors, such
as Apaf-1, Smac and cytochrome c. Therefore, the BH3-only and Bax family
members act in concert to tip the balance in the cell towards the apoptotic program
(reviewed in [15]). In our model, it was observed that deletion of Hrk did not rescue
the resorption phenotype; however, Bax KO embryos were protected from PAH-
induced death, as the proportion of Bax-deficient embryos was significantly higher in
PAH-treated, compared with vehicle-treated, Bax heterozygous females. Thus, Bax
appears to be a pro-apoptotic regulator of PAH-induced spontaneous abortion. In
addition, since Bax is a strong inducer of cell death, it is possible that the lack of
rescue seen in Hrk-deficient mice is due to overwhelming stimulation of Bax, and
that knocking out Hrk in such a model is insufficient to compensate for directly
activated Bax-driven death.
The results of our experiments indicate that maternal exposure to PAHs prior
to conception alters the sex ratio, with a significantly greater proportion of males per
litter being observed in PAH-treated compared with vehicle-treated dams.
Epidemiological studies examining the influence of cigarette smoke on human sex
143
ratios have yielded conflicting results, with reports of altered sex ratios at birth,
depending on the level of exposure, and whether the father or the mother, or both,
smoke tobacco products [395-397]; however, it was determined that exposure to
cigarette smoke does not appear to effect changes in the proportion of sperm
carrying either the X or Y chromosome [3897]. While the molecular mechanisms
behind sex skewing is unclear, it was recently reported that maternal smoking and
the genetics of signal transduction had an effect on the sex ratio at birth [398].
Additionally, alterations in the maternal sex hormone profile have been reported to
be associated with changes to the offspring sex ratio in rodents [399] and exposure
to BaP has been shown to affect sex hormone levels in pregnant rats [275].
Furthermore, female embryos may be more susceptible to apoptosis induction, as
several cell death associated genes (e.g. XIAP, AIF) are located on the X
chromosome and may impact the execution of Bax-mediated death. Hyperglycemia-
induced apoptosis of preimplantation embryos is a Bax-driven process [400] anda
recent report demonstrated differential susceptibility of male and female embryos to
apoptosis [401]; however, an increased number of viable female embryos was
observed in that study. Extrapolation of data from rodent-based studies to the
human population obviously requires extreme caution and the results of these
experiments merely underscore the need to continue investigations into the exact
relationship between cell death susceptibility, genetic sex and gene expression.
144
Conclusion
While many studies clearly indicate that antismoking interventions during
pregnancy should be a high priority as a part of prenatal care, exposure to PAHs
from second-hand smoke is more difficult to prevent. Moreover, even if women stop
smoking as soon as pregnancy is detected, this would not eliminate exposure to
PAHs, which have accumulated in maternal tissues and could still pose a significant
threat to the developing fetus. It is, therefore, important to dissect the molecular
mechanisms driving the biological effects of PAHs and develop strategies to
antagonize the adverse effects of toxic AhR ligands, as a step towards the future
design of therapies to improve fetal growth, development and survival.
145
CHAPTER 4
MATERNAL EXPOSURE TO POLYCYCLIC AROMATIC HYDROCARBONS
LEADS TO ALTERED PLACENTAL VASCULATURE AND IUGR IN C57BL/6
MICE, WHICH IS RESCUED BY AHR DEFICIENCY
146
CHAPTER 4: Maternal exposure to polycyclic aromatic hydrocarbons leads to altered placental vasculature and IUGR in C57BI/6 mice, which is rescued by AhR deficiency.
4.1 Abstract
Maternal cigarette smoking is considered to be an important risk factor
associated with fetal IUGR. Polycyclic aromatic hydrocarbons (PAHs) are well-
known constituents of cigarette smoke and the effects of acute exposure to these
chemicals at different gestational stages have been well established in a variety of
laboratory animals. In addition, many PAHs are known ligands of the aryl
hydrocarbon receptor (AhR), a cellular xenobiotic sensor responsible for activating
the metabolic machinery. In this study, we have developed a chronic, low-dose
regimen of PAH exposure to C57BI/6 mice prior to conception, which ultimately
resulted in IUGR in d15.5 fetuses. Furthermore, we observed both histological and
structural adaptations in the placental vasculature of PAH-exposed dams, with
significant reductions in arterial surface area and volume of the fetal vasculature in
d15.5 placentae. This altered vascularization was accompanied by reduced
labyrinthine and increased CP cell death rates. AhR-deficient fetuses were rescued
from PAH-induced growth restriction and exhibited no changes in the labyrinthine
cell death rate. The results of this investigation demonstrate that chronic exposure
to PAHs is a contributing factor to the development of IUGR in human smokers and
that the AhR pathway is involved.
147
4.2 Introduction
Cigarette smoking during pregnancy has serious consequences to maternal,
embryonic, fetal and neonatal health, having been associated with increased risks of
spontaneous abortion, placental abruption, placenta previa, ectopic pregnancy and
premature delivery (for reviews see [253, 360, 363]). Gestational exposure to
tobacco products is now causally associated with IUGR and is considered to be the
mediating factor in smoking-related neonatal mortality [402]. Only a small portion of
human smokers have growth-restricted babies and maternal genotype associated
with metabolism of polycyclic aromatic hydrocarbons (PAHs) has been implicated in
the development of this condition [403, 404].
While the direct cellular targets of cigarette smoke causing the IUGR
phenotype are unknown, maternal smoking has been reported to influence the
placental architecture, affecting both the vascular and trophoblast compartments.
Histomorphometric studies of placentae from smoking mothers have revealed
alterations in maternal villous spaces [263] and fetal capillary volume [262, 263, 265]
and surface area [265]. Functionally these changes are reflected by increased
resistance in both the uterine and umbilical arteries as determined by Doppler
Studies [264, 405]. In addition to alterations in placental vasculature, maternal
exposure to cigarette smoked has been associated with reduced ST apoptosis [266]
and trophoblast hyperplasia [406, 407].
There are greater than 4,000 chemical components found in cigarettes;
however, the main toxicants are a group of carcinogens known as polycyclic
148
aromatic hydrocarbons [408]. Included in this group are benzo(a)pyrene (BaP) and
dimethylbenz(a)anthracence (DMBA), which are known carcinogens and whose
toxic effects include the formation of DNA- and protein adducts, in addition to
triggering the expression of xenobiotic-metabolizing enzymes through binding to the
aryl hydrocarbon receptor (AhR). While PAHs are known environmental pollutants
generated by fossil fuel combustion, car exhaust and forest fires [409], or through
the consumption of smoked and grilled foods [410], the major source of human
exposure is through use of tobacco products [411]. Polycyclic aromatic
hydrocarbons have long been known to exert toxic effects on a variety of organs,
including those of the reproductive system (for review, see [412]). Furthermore,
PAHs have been shown to cross the placenta [413, 414] and form hemoglobin
adducts in both maternal and fetal sera [415], in addition to forming DNA adducts in
both human [272] and murine [416] trophoblasts.
The aryl hydrocarbon receptor (AhR) is a basic helix-loop-helix transcription
factor, acting as a xenobiotic sensor for a number of different hydrocarbons,
including PAHs (for review see [288, 367]). Ligands, such as BaP and DMBA,
diffuse across the cell membrane and bind to AhR, causing a conformational
change, exposing a nuclear localization sequence. This allows the receptor-ligand
complex to translocate into the nucleus, where it binds with its partner, the AhR
nuclear translocator (Arnt) and binds promoter regions at AhR/dioxin/xenobiotic
response elements (AREs/DREs/XREs), activating the transcription of cellular
detoxification machinery. AhR-deficient mice are resistant to BaP-induced
carcinogenicity [417],dioxin toxicity [290, 418], exhibit cardiac hypertrophy, reduced
149
fecundity and postnatal growth retardation, independent of exogenous ligand [291,
302]. AhR expression has been previously demonstrated in the mouse uterus and
fetal endothelium of the mouse placenta [293].
A number of murine studies have explored the consequences of acute dioxin
or PAH exposure during gestation [419-421]. In addition, laboratory studies have
revealed that rats exposed to side-stream smoke during pregnancy yielded pups
with significant decreases in weight [422, 423]. However, there is little information
regarding the effect of maternal exposure to PAHs prior to pregnancy. As these
chemicals have been shown to accumulate in the adipose and mammary tissue
[279, 424], the slow release of unaltered PAHs into the maternal blood can still
present a toxicological threat to the growing fetus. We previously reported a murine
model [425] designed to mimic the phenomenon observed in human populations,
where women will cease smoking upon attempting, or acquiring knowledge of,
conception — typically due to fetal health concerns [373, 374]. Herein, we report that
chronic exposure to PAHs prior to gestation, results in compromised maternal and
fetal placental vascularization and altered labyrinthine architecture in C57BI/6 mice,
leading to |UGR, which is rescued by AhR deficiency.
4.3 Materials and Methods
4.3.1: In vivo BaP and DMBA treatment
C57BI/6 (National Cancer Institute, Frederick, Maryland, USA) and AhR
heterozygous (C57BI/6-AhR”"*") virgin female mice were randomly separated into
PAH-treated or vehicle-treated groups and group-housed in separate cages.
150
Animals were maintained in a controlled room with a 12h light: 12 h dark cycle and
allowed ad libitum access to rodent chow and water. Subcutaneous injections of
vehicle or PAHs were administered over a nine-week period as previously described
[425]. The final, cumulative dose for PAH-treated mice was 12 mg/kg; vehicle-
treated animals were given proportional injections of corn oil, according to body
weight.
4.3.2: Mating and tissue collection
Four days after the last injection, female mice were mated with the
appropriate male stud (i.e. C57BI/6 or AhR Het males). Gestational age was
determined based on the presence of a vaginal plug, with the morning of detection
designated as day 0.5 (d0.5) post coitum. Plugged females were removed from the
male and group-housed in separate cages; it was ensured at all times, that PAH-
treated and vehicle-treated females were placed in different cages. Pregnant dams
were euthanized by cervical dislocation at d15.5 and uteri were placed in phosphate-
buffered saline (PBS; the number of conceptuses and resorptions was recorded.
Fetal and placental wet weights were taken and placentae derived from AhR
heterozygous mothers were halved at the approximate midline. The larger half
containing the umbilicus was fixed in ice-cold, 10% phosphate-buffered formalin and
the smaller half was frozen on dry ice. C57BI/6 placentae were fixed or frozen
whole. Where required, a piece of fetal forelimb tissue was removed, washed in
PBS, placed on dry ice and stored at -20°C for PCR genotyping. Frozen tissue was
151
stored at -80°C and fixed tissue was washed twice for 1 hour in PBS and stored in
70% ethanol at 4°C. AhR fetuses were genotyped by PCR as previously described
[301]. All animal experiments were conducted using protocols approved by the
Animal Care Committee at the Samuel Lunenfeld Research Institute, Mount Sinai
Hospital.
4.3.3: Vascular casting and ultrasound biomicroscopy
Vehicle- and PAH-exposed, C57BI/6 pregnant dams were euthanized by
cervical dislocation at d15.5 and vascular casts were made with methyl methacrylate
(i.e. plastic) casting compounds and processed for scanning electron microscopy
(SEM) using established methods [150]. This technique was used to qualitatively
examine the fetal and maternal placental circulations. Briefly, plastic casts of the
feto-placental circulation were obtained by dissecting d15.5 pregnant uteri and
placing tissue into ice-cold PBS. Concepituses were individually exposed and placed
in a warm saline bath to inititate cardiac function and placental blood flow. After
inserting a glass cannula into either the umbilical vein or artery, blood was flushed
from the placental circulation with warmed saline (0.9% NaCl, 2% xylocaine, 100 IU
heparin/mL). Methyl methacrylate casting compound (Polysciences Inc.,
Warrington, PA; Batson’s number 17; 5 mL monomer base, 1.5mL. catalyst, 0.1 mL
promoter) was infused into one umbilical vessel until it exited via the other, inn order
to completely fill the feto-placental vasculature. The vessels were tied off and the
casting compounds were allowed to polymerize for several hours, after which the
152
placenta was severed from the fetus. To remove surrounding tissue, placentae were
immersed in 20% KOH and casts were subsequently washed with water and air-
dried.
Plastic casts of maternal placental circulations were obtained by euthanizing
d15.5 pregnant mouse by cervical dislocation and injecting 50 wL of 100 IU/mL
heparin into the still-beating heart. The chest was opened and a catheter inserted
into the descending aorta; a cut was made into the right atrium to serve as an exit for
the perfusate. The initial perfusate consisted of chilled saline-xylocaine mixture (as
described previously), which dilated the vessels and cleared the circulation of blood.
This was followed by injection of approximately 4-5 mL of liquid plastic (prepared as
described previously), after which the inferior vena cava was ligated. Once the
plastic hardened, the uterus was removed and cut between the individual
implantation sites. Casts were exposed by digesting the surrounding tissue with
KOH, washing with water and air-dried, as described previously. Plastic casts for
both fetal (Nvenicie=4 placentae from 2 dams; nean=5 placentae from 2 dams) and
maternal (Nvehicie=3 placentae from 2 dams; npay=3 placentae from 2 dams) placental
circulations were viewed using a FEI XL30 (FEI Systems Canada Inc., Toronto, ON)
scanning electron microscope.
Microcomputed tomography (MicroCT) was employed to obtain quantitative
measurements of the feto-placental vasculature, using methods previously
described [336]. Briefly, d15.5 pregnant uteri were collected into ice-cold PBS.
Conceptuses were individually exposed and placed in a warm saline bath to inititate
cardiac function and placental blood flow. After inserting a glass cannula into either
153
the umbilical vein or artery, blood was flushed from the placental circulation with
warmed saline (0.9% NaCl, 2% xylocaine, 100 IU heparin/mL). Radio-opaque
silicone rubber (Microfil, Flow Technology, Carver, MA, USA) was infused into the
vessels until it reached the capillaries. The vessels were tied off and the casting
compounds were allowed to polymerize for several hours, after which the placenta
was severed from the fetus. The perfused placenta was fixed in 10% phosphate-
buffered formalin and mounted in 1% agar containing 10% formalin for subsequent
scanning. Three-dimensional data sets were obtained using an MS-9 micro-CT
scanner (GE Medical Systems, London, ON, Canada) and analyzed using Amira
software (TGS, Berlin, Germany). Images and data were obtained for both arterial
(Nehicile=9 placentae from 4 dams; npay=9 placentae from 4 dams) and venous
(Nvehicle=8 placentae from 4 dams; npay=8 placentae from 4 dams) fetal vessels.
Ultrasound biomicroscopy (UBM) was utilized to assess placental
hemodynamics and fetal dimensions in vivo. Vehicle-exposed and PAH-exposed
dams were anaesthetized with isofluorane at d15.5 and crown-rump length, fetal
heart rate and pulse velocity of the uterine artery were measured using 30 MHz
ultrasonography (Vevo 770, Visualsonics, Toronto, ON, Canada). Data were
obtained for 11-15 fetuses from three vehicle-exposed dams and 17-19 fetuses from
four PAH-exposed dams.
4.3.4: Terminal deoxynucleotidyl transferase dUTP nick-end labeling
C57BI/6, AhR wildtype (WT) and AhR knockout (KO) placentae from vehicle-
or PAH-exposed dams were embedded in paraffin using routine histological
154
techniques and 5 um sections were taken at the midline. Sections were
deparaffinized and were labeled, and TUNEL-labelled cells were quantified using
techniques similar to those described in section 2.3.2.
4.3.5: Histological Staining
Sections were deparaffinized in xylene and rehydrated to water. To
distinguish cytotrophoblast cells lining the maternal blood spaces, rehydrated
sections were briefly equilibriated with alkaline phosphatase (AP; 100 mM Tris, 100
mM NaCl, 5 mM CaCh, pH 8.5) buffer, then held in AP substrate solution (NBT +
BCIP in AP buffer; Promega, Madison, WI, USA) for 25 minutes at 37°C ina
humidified chamber. Slides were washed briefly with water, stained with nuclear fast
red and counterstained with 1% tartrazine yellow. To visualize collagen deposition,
Masson’s trichrome stain was applied, after post-fixing rehydrated sections in
Zenker’s fixative for 1 hour.
4.3.6: Immunohistochemistry and Lectin Histochemistry
Sections were deparaffinized in xylene, rehydrated and underwent microwave
antigen retrieval in 10 mM citrate buffer (pH 6.0). Subsequent steps were performed
in the same manner as those described in section 2.3.4, using anti-AhR antibody
(1:500; Biomol, Plymouth Meeting, PA, USA). The techniques used for lectin
histochemistry are also described in section 2.3.4.
155
4.3.7: Caspase-3 enzyme assay
Enzymatic activity of caspase-3 in vehicle- or PAH-exposed C57BI/6
placentae was assessed using the Caspase-3 Cellular Activity Assay Kit PLUS
(Biomol, USA), as described in section 2.3.5
4.3.8: Western blotting
To assess protein expression in control or treated C57BI/6 placentae, one
placenta from each of five dams was processed as described in section 2.3.6.
Individual AhR WT and KO placentae (vehicle and PAH-exposed) were similarly
treated, after maternal decidua was removed. Polyacrylamide gels and immunoblots
were prepared as previously described (Section 2.3.6) and the following primary
antibodies were used: anti-caspase-3 and -6 (1:500; Cell Signalling, Danvers, MA,
USA); anti-cleaved Parp-1 (1:500, Cell Signalling); anti-Bax NT (1:500, Upstate,
Lake Placid, NY, USA); anti-Xiap (1:500, BD Biosciences, Mississauga, ON,
Canada); anti-FasL (1:200; Santa Cruz Biotechnology, Santa Cruz, CA, USA); p53
(Vector labs, Burlington, ON, Canada); anti-FAK (Santa Cruz); and, p21
(Calbiochem, Mississauga, ON, Canada). Blots were stripped and reprobed with
anti-B-actin antibody (1:400, Santa Cruz) to correct for protein loading.
4.3.9: Statistical analysis
Statistical analysis of AnR data was done using two-way ANOVAs. All other
statistical tests were done using Student's t-test. Statistical software used was
SPSS® (Version 13) and data were considered statistically significant if p < 0.05.
156
4.4 Results
4.4.1: Maternal exposure to PAHs prior to conception leads to IUGR and altered labyrinthine vasculature in C57BI/6 mice
We have previously shown that maternal exposure to PAHs prior to
pregnancy on an outbred, ICR genetic background results in increased resorption
rates due to elevated cell death during the preimplantation stage [425]. While
C57BI/6 dams exposed to PAHs exhibited a trend towards smaller litters, this
decrease was not statistically significant (data not shown). Instead, PAH treatment
of C57BI/6 females yielded fetuses with a 14% reduction in weight compared to
fetuses from dams exposed to vehicle (Figure 4.1a). These data were supported by
crown-rump length measurements by UBM, which were significantly reduced in
fetuses from PAH-exposed dams (Figure 4.1b).
Evaluation of d15.5 placental sections using various histological techniques
revealed aberrations in the labyrinthine region, particularly in the vasculature. After
staining placental sections from PAH-exposed dams with Masson’s trichrome, it was
apparent that collagen deposition along the chorionic plate and into the large
chorionic vessels was thinner than in vehicle-treated controls (Figure 4.1c). In
addition, alkaline phosphatase and lectin (BS-l) histochemistry (markers of maternal
and fetal blood spaces, respectively) revealed alterations in the labyrinthine
architecture, characterized by dilatation of both the maternal blood spaces and fetal
microvasculature (Figure 4.1c). The other placental regions were examined but did
not exhibit any obvious defect.
157
Figure 4.1 Maternal exposure to PAHs prior to conception leads to IUGR and
altered labyrinthine architecture in C57BI/6 mice at d15.5 gestation. A. Bar
graph depicts placental and fetal weight of d15.5 conceptuses from C57BI/6 dams
exposed to vehicle (n=62 conceptuses from 8 dams) or PAHs (n=55 conceptuses
from 9 dams) prior to pregnancy. B. Graph demonstrates fetal crown-rump length
measurements of d15.5 fetuses from vehicle-exposed (n=15 fetuses from 3 dams)
and PAH-exposed (n=17 fetuses from 4 dams) dams. C. Photomicrographs in
upper panel represent the basolateral edge of d15.5 placentae, exposed to vehicle
or PAHs and stained with Masson’s trichrome (nuclei are dark red-blue, cytoplasm is
red, collagen is bright blue). Photomicrographs in middle panel are of d15.5
placental labyrinth obtained from vehicle- or PAH-exposed dams, after histochemical
Staining with alkaline phosphatase (AP) and counterstaining with nuclear fast red
and tartrazine yellow. Purple-staining outlines the maternal blood spaces due to
fetal CTB reaction with AP substrate, cytoplasm is yellow or yellow-orange and
nuclei are red. Lower panel contains photomicrographs of d15.5 C57BI/6 labyrinth
exposed to vehicle or PAHs and labeled with Bandeiraea simplicifolia (BS-l) lectin (a
marker of endothelial cells), outlining the fetal blood spaces; nuclei are
counterstained with hematoxylin. Bars represent mean values + standard error (SE)
and values of significant statistical difference are shown with the corresponding p
value. Arrows indicate the line of collagen deposition at the chorionic plate and
arrowheads indicate chorionic vessels.
158
A. d15.5 Fetal and Placental Weights B. Fetal Crown-Rump Length Measurements by UBM
0.5 p<0.001 y
0.45 14
— 0.4
S 0.35 0 Vehicle = 138 £ 03 m PAHs = 13.6 g 0.25 13.4
0.2 D 13.2 “ % 13.0
0.05 _ 12.8 _
o |ins82 12.6 n=15 Placental Weight Fetal Weight Vehicle PAHs
C. Vehicle
Masson’s trichrome for
collagen
Alkaline phosphatase for CTBs lining maternal blood
spaces
BS-I for
fetal blood
spaces
Figure 4.1
159
To qualitatively evaluate the 3-D changes induced by maternal exposure to
PAHs, plastic vascular casts of the maternal and fetal placental circulations were
prepared. Consistent with those alterations observed in histological sections,
placental vascular casts revealed several changes in the vascular tree. Casts of the
fetal placental vasculature from mothers treated with PAHs, consistently exhibited
engorged, dilated capillaries that were not evident in the feto-placental casts from
dams exposed to vehicle (Figure 4.2a, b). Additionally, PAH-exposed fetal
capillaries exhibited numerous, intricate anastomoses and a greater degree of
tortuosity compared with the more linear structures observed in the fetal casts
exposed to vehicle. Moreover, this same dilatation and engorgement was apparent
in the maternal placental canals of PAH-exposed placentae (Figure 4.3a, b). Lastly,
large maternal canals were consistently observed to be projecting out of the
junctional zone, close to the chorionic surface of placentae obtained from dams
treated with PAHs (Figure 4.3b).
4.4.2 Reduced umbilical vessel diameter and total fetoplacental vascular surface area and volume in d15.5 placentae from PAH-exposed dams
Micro-computed tomography (microCT) was employed to measure all feto-
placental vessels greater than 0.03mm in diameter, with 3-D datasets and iso-
intensity surface renderings acquired as previously described [336]. The acquired
160
Figure 4.2 Maternal exposure to PAHs prior to conception in C57BI/6 mice
results in aberrant placental microvasculature in the fetal compartment.
Scanning electron photomicrographs of corrosion casts viewed from the chorionic
side from (A) vehicle and, (B) PAH-exposed d15.5 C57BV6 placentae. Boxed region
in cast of feto-placental vasculature in upper-left panel is magnified in centre panel.
Boxed regions in centre panel are magnified in panels to the right.
162
Figure 4.3 Maternal exposure to PAHs prior to conception in C57BI/6 mice
results in aberrant morphology of blood spaces in maternal compartment.
Scanning electron photomicrographs of corrosion casts of maternal placental
labyrinthine canals from (A) vehicle and (B) PAH-exposed d15.5 C57BI/6 placentae.
Boxed region in left panel is magnified in right panel. Arrow indicates a large,
superficial maternal canal. Superficial canals were consistently observed in
maternal-side casts obtained from PAH-exposed dams.
164
surfaces (see Figure 4.4a, c) allowed 3-D visualization of the fetoplacental
vasculature as well as calculation of vessel diameters, surface area, and overall
lumen volume. While no overt changes in the large vessels of the venous
vasculature were observed between vehicle and PAH-exposed placentae, the
arterial surface renderings of PAH-exposed placentae displayed a greater degree of
tortuousity in some large vessels of the trees (Figure 4.4b). In addition, PAH-
exposed placentae exhibited significantly reduced arterial surface area and volume
compared to placentae from vehicle-exposed dams (Figure 4.5a, b), while no
change in venous surface area or volume was observed between the two groups.
However, both the umbilical artery and vein demonstrated significant decreases in
diameter in placentae from dams treated with PAHs compared to dams treated only
with vehicle (Figure 4.5c). In spite of these alterations in fetal and placental
vasculature, fetal abdominal cross-sectional area, fetal heart rate and the peak
systolic blood velocity in the umbilical artery did not change with PAH exposure, as
determined by Doppler studies (Figure 4.6a-c).
4.4.3 Both fetal and maternal compartments of d15.5 PAH-exposed placentae exhibit altered cell death rates and changes in cell death markers
Polycyclic aromatic hydrocarbons have been implicated in altering the
balance of cell survival and death in a number of different cell types [864, 426, 427].
As precisely regulated cell death is essential for trophoblast turnover, analyses of
cell death were implemented. Morphometric analyses of d15.5 placental sections
after TUNEL, revealed significant decreases in the number of labeled cells in the
165
Figure 4.4 Two-dimensional renderings of d15.5 fetal placental vessels from
vehicle and PAH-exposed dams, after micro-computed tomography. A. Two-
dimensional rendering of fetal arterial cast obtained from d15.5 placentae of vehicle
and PAH-exposed dams. B. Higher magnification of boxed region in (A)
demonstrating the altered curvature of the larger fetal vessels. Red arrows indicate
the direction of blood flow. C. Two-dimensional rendering of fetal venous cast
obtained from d15.5 placentae of vehicle and PAH-exposed dams.
166
MICRO-COMPUTED TOMOGRAPHY OF d15.5 FETAL PLACENTAL VESSELS UP TO 13 um RESOLUTION
A. Vehicle PAH-exposed
Arterial
Cast
Venous
Cast Figure 4.4
167
Figure 4.5 Micro-computed tomography of fetal placental casts reveals
decreased arterial surface area and umbilical vessel diameter in placenta from
PAH-exposed C57BI/6 dams. A. Graph depicting the average surface area of the
fetal, arterial or venous vasculature in vehicle and PAH-exposed placentae. B.
Graph depicting the average fetal, arterial or venous volume in vehicle and PAH-
exposed placentae. C. Graph depicting the average fetal arterial or venous
umbilical vessel diameter in vehicle or PAH-exposed placentae. Bars represent
average values + SE and values of significant statistical difference are shown with
the corresponding p value (Student’s t-test).
168
A. Vascular Surface Area
_ 120, p=0.0043 N
E 100 - | D Vehicle 80 - m@ PAHs
g 60 -
8 40 -
“© 204 > YM 4 n=9 n=8
Arterial Venous
B. Vascular Volume
4 - p=0.0032
3.5 +
E 3 | | & 2.54 D Vehicle
@ 24 m@ PAHs
E 1.54 6 1- >
0.5 4 0 n=9 n=8
Arterial Venous
C. Umbilical Vessel Diameter
06- | p=0.00014 3=0.00074
—~ 0.54 | E Oo i € 0.44 Vehicle
_ @ PAHs £2 034
reby
— 02] QO
0.1 -
0 n=9 n=7
Arterial Venous
Figure 4.5
169
Figure 4.6 Chronic exposure to PAHs prior to conception does not alter fetal
heart rate, abdominal cross-sectional area, nor umbilical artery pulse velocity,
as determined by ultrasound biomicroscopy. Graphs depict unchanged (A)
abdominal cross-sectional area in d15.5 fetuses; (B) heart rate in d15.5 fetuses; and
(C) pulse velocity of the umbilical artery, after maternal exposure to PAHs. Bars
represent average values + SE; n values reflect the number of fetuses analyzed in
vehicle (n=3) and PAH-exposed (n=4) dams.
Peak velocity (m
m/s)
Ar
ea (mm?)
Rate
(b
eats
pe
r minute)
35
30
25
250
200
150
100
50
20)
15]
10}
170
Abdominal Cross-sectional Area
n=11
Vehicle PAH-exposed
Fetal Heart Rate
n=14
Vehicle PAH-exposed
Peak Systolic Blood Velocity in the Umbilical Artery
o
zr
>
ON
[SP 6 O
o N
<A Oo
oOo
oO
n=14
Vehicle PAH-exposed
Figure 4.6
171
labyrinth and junctional zone of placentae from PAH-exposed dams (Figure 4.7a).
Based on the location and the presence of fetal red blood cells, the dead/dying cells
appear to be a combination of fetal endothelium and ST cells. In addition, the
incidence of sporadic decidual cell death, and the percent area of TUNEL-positive
tissue in the maternal compartment also significantly decreased compared with
placentae exposed to vehicle only (Figure 4.7a, b). Conversely, PAH treatment
caused a significant increase in the number of TUNEL-positive cells in the CP
(Figure 4.8a), whereas TGCs remained unaffected (Figure 4.8b). Note that positive
(section pre-incubated with DNase | enzyme) and negative (sections incubated
without Tdt enzyme) controls exhibited high levels and absence of TUNEL-positivity,
respectively
Assessment of cell death markers revealed altered expression and activity in
several key proteins. Decreased rates of placental cell death in dams exposed to
PAHs were accompanied by diminished caspase-3 enzyme activity (Figure 4.9a).
These data were supported by immunoblotting, as levels of cleaved caspase-3 and -
6 also declined significantly, while total caspase-3 and -6 levels appeared
unchanged (Figure 4.9b, c). Moreover, examination of the cleavage profiles of
known, intracellular caspase-3 substrates [93, 324, 325] revealed significantly
reduced levels of the cleaved forms of Parp-1 (Figure 4.10a), p21 (Figure 4.10b),
PTEN (Figure 4.10c) and FAK (Figure 4.10d). Additionally, Bax, a pro-apoptotic
protein known to be regulated by AhR after PAH exposure [370] exhibited
significantly decreased levels of expression in placentae from PAH-exposed,
compared with vehicle-exposed dams (Figure 4.11a). Moreover, significantly higher
172
Figure 4.7 Chronic exposure to PAHs prior to pregnancy leads to altered cell
death patterns in d15.5 placentae of C57BI/6 dams. A. Graph depicts the
number of TUNEL-positive nuclei per 100 ym? of labyrinthine, junctional zone or
decidual tissue in d15.5 vehicle or PAH-exposed placentae. Data for decidual cells
reflect positive cells sporadically placed within the maternal compartment.
Accompanying photomicrographs in right panel represents TUNEL patterns
observed in vehicle or PAH-exposed placental labyrinth. B. Graph depicts the
percent area of tissue in the maternal compartment that was regions of clustered
TUNEL-positive cells. Accompanying photomicrographs in right panel demonstrates
foci — demarcated with dashed line — of TUNEL-positive cells in the maternal
compartment. Arrows indicate TUNEL-positive nuclei and empty arrowheads
specify trophoblast giant cells in the fetal compartment. Bars represent average
values + SE and values of significant statistical difference are shown with the
corresponding p value (Student's t-test).
#TUNEL-positive
cells
2 per
100
pm
Percent
area
of Maternal
# TUNEL-positive cells
18 p=0.03
1:2 © Vehicle
1.0) p=0.0046 m PAHs 0.8
0.6
0.2
0 n=8 [li Labyrinth Junctional Decidua -
Zone sporadic death
Percent Area of Maternal Compartment
that is TUNEL-postive foci
3.5
3.0
25
2.0
1.5
1.0
°° nin Vehicle PAH-treated
-positive
(%)
Compartment
that
is TUNEL
173
Vehicle PAH-exposed
ne Ss ¥ ins atk
Foci of TUNEL-positive cells in maternal compartment - d15.5 midline placenta
Figure 4.7
174
Figure 4.8 Chronic exposure to PAHs prior to pregnancy leads to increased
chorionic plate cell death, but TGC death is unaffected. A. Graph depicts the
number of TUNEL-positive nuclei per 100 wm? of CP in d15.5 vehicle or PAH-
exposed placentae. Accompanying photomicrographs in right panel demonstrate
TUNEL staining observed in vehicle or PAH-exposed CP. B. Graph depicts the
percentage of TUNEL-positive or condensing TGC, or the percentage of TGC
containing TUNEL-positive corpses. Arrows indicate TUNEL-positive nuclei. Bars
represent average values + SE and values of significant statistical difference are
shown with the corresponding p value (Student’s t-test).
e,cells
per
100
pm
#TUNEL-positiv
175
#TUNEL-positive Chorionic Plate Cells PAH-exposed
35 p=0.03 | 3.0 5 0 5
r
n=8
Vehi PAH- —— * ehicle treated Chorionic plate - d15.5 midline placenta
B. Rates of TGC death due to. PAH Exposure
16
. 14 ey GS 12
© § 40 C1 Vehicle
m= oO m PAH-exposed o DM
ao? 8 Do fe 6 a 8 Po 4 oo
a. 2
0 n=8 i % TUNEL-positive. .. % condensed %TGC with
TGC TGC TUNEL-positive
corpses
Figure 4.8
176
Figure 4.9 Chronic exposure to PAHs prior to conception disrupts the
expression levels of executioner caspases in d15.5 C57BI/6 placentae. A.
Graph demonstrates the average caspase-3 enzyme activity levels in 50 yg of
placental lysate obtained from d15.5 vehicle or PAH-exposed dams. Representative
immunoblots are shown to the right of each graph. Bars represent average values +
SE and values of significant statistical difference are shown with the corresponding p
value (Student's t-test).
Densitometric
rati
o of
total
caspase-6:actin
Densitometric
ratio
2 o
0.5
0.4
0.3
0.2
© QO
177
A. Caspase-3 Enzyme Assay - d15.5
Placental Lysates
S ° O Vehicle Ee 6 | m™ PAH exposed Es
se 8 Eo 4 £2 3 28 5 p=0.025
2 1 0 n=5
Vehicle PAH-exposed
Caspase-3 Expression
p=0.029 35 kDa Procaspase-3
0.45
0.4 038 18 kDa Cleaved Caspase-3
0.2 0.2 = Se =) actin
Vehicle PAH- 0.1 _ = 0.0 n=6 N=6 exposed
0 — | Total Caspase-3: Cleaved Caspase-3:
actin total caspase-3
Caspase-6 Expression
35 kDa Procaspase-6
p=0.041 0.025 g g
UD =
0.02 88 9 o
0.015 2 15 kDa Cleaved , go Caspase-6
» 2 0.10 os
@ 9, Bo
v 0.005 oa Vehicle PAH- c Qo S$ exposed
a
Total Caspase-6: Cleaved Caspase-6:
actin Total Caspase-6
Figure 4.9
178
Figure 4.10 Cleavage levels of active caspase-3 cellular substrates are
reduced in d15.5 PAH-exposed placentae. Graphs demonstrate levels of cleaved
(A) Parp-1; (B) p21; (C) PTEN; and, (D) FAK, in d15.5 placental lysates from
vehicle- or PAH-exposed dams. Representative immunoblot bands for vehicle and
PAH-treated placental lysates are depicted alongside corresponding graphs. Bars
represent average values + SE and values of significant statistical difference are
shown with the corresponding p value (Student’s t-test).
5 g 0.025
2 0.020 a
© 0.015 2 a.
6 ® 0.010 = > nO
53 0.005
0
3X 0:6
ok 05 oH ef 0:4
ge 0.3
on a © 0.2
gs 0.1
0
0.05 OQ QF 0.04 © £ 22 0.03 @aa
53 0.02 a>
= 8 0.01 oOo
0
0.86
0.84
0.82 0.8
0.78
0.76
0.74
0.72 Densitometric
rati
o of
cleaved
PTEN:total PTEN
Cleaved Parp-1 (70 kDa)
+
p=0.044
n=3 n=3
Vehicle PAH-exposed
Levels of Caspase-3-specific Cleaved FAK
p=0.015
n=5 Vehicle PAH-exposed
Levels of Caspase-3-specific Cleaved p21
p=0.005
n=5
125 kDa
Vehicle PAH-exposed
Levels of Caspase-3-specific Cleaved PTEN
p=0.026
n=5
Vehicle PAH-exposed
30 kDa
179
cleaved Parp-1
" &-actin
Vehicle PAH- exposed
Vehicle
21 kDa
14.kDa
Vehicle
Vehicle
yj) Full-length FAK
cleaved FAK
PAH- exposed
#| Full-length p21
| cleaved p21
PAH-
exposed
=| Full-length PTEN
kj} cleaved PTEN
PAH- exposed
Figure 4.10
180
Figure 4.11 Chronic exposure to PAHs prior to conception disrupts the
balance of apoptotic and anti-apoptotic proteins in d15.5 C57BI/6 placentae.
Graphs demonstrate the levels of (A) Bax; (B) Xiap and, (C) FasL, as assessed by
immunoblotting, in d15.5 placental lysates from vehicle or PAH-exposed dams.
Representative immunoblots are shown to the right of each graph. Bars represent
average values + SE and values of significant statistical difference are shown with
the corresponding p value (Student’s t-test).
Densitometric
ratio
Densitometric
rati
o of
Densitometric
ratio
of FasL:actin
Bax:actin
0.2
0.15
0.1
0.05
of Xi
ap:a
ctin
oOo NM
FF
DD.
a
cn &
oo
=
tn
Nb
oO
oO a
181
Bax Expression
T 21 kDa oom! Bax
p=0.044 Vehicle PAH-
exposed
n=5
Vehicle PAH-exposed
Xiap Expression
p=0.042
i) [eed] | Xiap
i (we) (wwe! §=—R-actin
Vehicle PAH-
exposed
n=5
Vehicle PAH-exposed
FasL Expression
p=0.023
H FasL R-actin
Vehicle PAH-
exposed x
n=3
Vehicle PAH-exposed
Figure 4.11
182
expression levels of Xiap, an anti-apoptotic protein, were observed in placentae from
PAH-treated dams (Figure 4.11b). Lastly expression levels of FasL, also known to
be regulated through AhR [428] and shown to be cytoprotective in endothelial cells
[429, 430], was increased in response to PAH exposure in d15.5 placental lysates
(Figure 4.11c).
4.4.4 AhR-deficient fetuses are protected from IUGR due to chronic maternal exposure to PAHs
The aryl hydrocarbon receptor acts as an intracellular sensor, triggering the
transcription of cellular machinery and initiating the appropriate response against
potentially harmful xenobiotics. Levels of AnR expression as determined by
immunoblotting and immunohistochemistry, exhibited a small, but significant,
increase in WT placentae from PAH-exposed dams (Figure 4.12a). Furthermore,
immunoblotting and densitometric analyses of PAH-exposed placental lysates
exhibited significantly increased levels of AnR-regulated p53 [431] and its
downstream target, p21 (Figure 4.12b,c). To ascertain which placental cell types
express AhR, immunochistochemistry was performed on d15.5 placental sections.
AhR immunolocalized to the maternal endothelial cells of the decidua and to the fetal
endothelium of the labyrinthine, chorionic plate and vitelline vessels. This staining
pattern was specific, as it was not evident in the placentae of AhR KO littermates
(Figure 4.13a).
AhR heterozygous dams exposed to PAHs prior to conception yielded AhR
WT and Het offspring exhibiting a significant decrease in weight compared with
vehicle-exposed fetuses; however, PAH-exposed AhR KO fetuses demonstrated no
183
Figure 4.12 Chronic exposure to PAHs prior to conception up-regulated AhR
expression and known target genes of AhR in C57BI/6 placentae. Graphs
depict expression levels of (A) AhR; (B) p53, and (C) p21 protein in d15.5 placental
lysates from vehicle or PAH-exposed dams. Representative immunoblots are
shown to the right of each graph. Bars represent average values + SE and values of
significant statistical difference are shown with the corresponding p value (Student’s
t-test).
Densitometric
rati
o of
p53:actin
Densitometric
ratio
of Ah
R:ac
tin
Dens
itom
etri
c ra
tio
of p21:actin
0.35
0.3
0.25
0.2
0.15
0.1
0.05
184
AhR Expression
p=0.022
n=5
0.5 5
0.45 -
0.4 4
0.35.4
0.3 4
0.25 +
0.2 4
0.15 +
0.1 4
0.05 ;
Vehicle PAH-exposed
p53 Expression
p=0.024
FH p53
Vehicle PAHs
n=3
0.06
0.05
0.04
0.03
0.02
0.01
Vehicle PAH-exposed
p21 Expression
p=0.021
p21
R-actin
Vehicle PAHs
Vehicle PAH-exposed
Figure 4.12
185
Figure 4.13 Aryl hydrocarbon receptor is expressed in the fetal endothelium
of the mouse placenta and AhR deficiency rescues the IUGR phenotype in
dams chronically exposed to PAHs prior to conception. A. Photomicrographs
of d15.5 AhR WT (upper left and right panels) and AhR KO (lower left and right
panels) placenta after immunohistochemica! staining with anti-AhR antibody. Fetal
endothelial cells in the labyrinth are indicated by arrows while those of the CP are
indicated by a ¢. Asterisks specify maternal blood spaces. B. Graph exhibits d15.5
weight in AnR WT, Het and KO fetuses from heterozygous dams exposed to vehicle
(n=5 dams) or PAHs (n=9 dams) prior to conception. Bars represent average values
+ SE and values of significant statistical difference are shown with the corresponding
p value (Tukey-Kramer test).
Weight
(g)
AhR KO Labyrinth
186
Fetal Weight
AhR KO
06- p=0.036 p=0.0092
0.5 | | | O Vehicle 0.4: lm PAH-exposed 0.3 4
0.2 4
o1/ |S © = i i i
0 | Cc Cc
AhR WT AhR Het AhR KO
Figure 4.13
187
further restriction in growth compared with KO offspring from dams exposed to
vehicle only (Figure 4.13b).
The aryl hydrocarbon receptor has been implicated in a number of different
cellular pathways, including cell death, survival and the cellular stress response.
While expression of the proliferation marker, Ki67, was not obviously altered
amongst vehicle- and PAH-exposed placental sections in both AhR WT and KO
placental sections (Figure 4.14), levels of several cell death markers differed in all
four groups of placental lysates. In the absence of PAHs, placental lysates from
AhR KO fetuses exhibited statistically significant increased levels of cleaved
caspase-3 compared with placental lysates from WT littermates (Figure 4.15a).
After chronic, maternal exposure to PAHs, significantly decreased levels of cleaved
caspase-3 were observed in both PAH-exposed AhR WT and KO placental lysates.
Morphometric analyses of TUNEL-stained placentae from AhR WT and KO
littermates of dams exposed to vehicle or PAHs, revealed a reduction in labyrinthine
cell death rates of PAH-exposed, AhR WT placentae, which was not evident in AhR
KO placentae (Figure 4.15b). Lastly, both AnR WT and KO placentae from PAH-
exposed females demonstrated significantly higher numbers of TUNEL-positive cells
in the CP, compared with that seen in AhR WT and KO placentae from dams treated
with vehicle.
188
Vehicle PAH-exposed
AhR KO eee
Ki-67 immunohistochemistry on d15.5 labyrinth
Figure 4.14 Maternal exposure to PAHs does not alter proliferation in d15.5
C57BI/6 placentae, as evidenced by Ki-67 immunohistochemistry.
Photomicrographs in upper panel represent d15.5 AhR WT labyrinth after Ki67 IHC
from vehicle (left panel) and PAH-treated (right panel) dams. Photomicrographs in
lower panel represent d15.5 AhR KO labyrinth after Ki67 IHC from vehicle (left
panel) and PAH-treated (right panel) dams.
189
Figure 4.15 Maternal exposure to PAHs results in altered cell death rates in
different regions of C57BI/6 placentae. A. Graph depicts levels of total and
cleaved caspase-3 in d15.5 fetal-enriched, AR WT or KO placental lysates from
vehicle or PAH-exposed AhR heterozygous dams. Representative immunoblots are
shown below graph. B. Graph depicts the average number of TUNEL-positive cells
per 100 pm? of labyrinthine or CP tissue in d15.5 AhR WT or KO placentae from
dams exposed to vehicle or PAHs. Bars represent average values + SE and values
of significant statistical difference are shown with the corresponding p value (Tukey-
Kramer test).
> Densitometric
ratio
of cleaved
Procaspase-3 >
Cleaved caspase-3
#TUN
EL-p
osit
ive
cell
s
caspase-3:total
casp
ase-
3 2
per
100
um
190
Cleaved Caspase-3
p=0.027 p=0.026
0.30 || 0.25 4
0:20 p=0.038
0.15 | |
0.10
~ n=3 n=3
AhR WT AhR KO
Vehicle PAHs Vehicle PAHs
4.0
3.5
3.0 2.5 2.0
1.5]
1.01
0.5)
AhR WT
33 kDa
+17 kDa
AhR KO
TUNEL data for d15.5 AhR Placentae
p=0.00013
oe
p=0.045
p=0.013
AhRWT AhRKO
«<— Labyrinth —»
AhRWT AhRKO
«<— Chorionic Plate —
Figure 4.15
191
4.5 Discussion
Cigarette smoking during pregnancy is linked with a number of detrimental
outcomes, and has now been established to be causally associated with IUGR. We
recently reported the development of a new animal model of pre-pregnancy
exposure to PAHs, which on an outbred genetic background (ICR) compromises
preimplantation development, leading to embryonic resorptions [425]. The
mechanism by which PAHs exert this phenotype involves the induction of cell death
in a Bax-dependent manner, as Bax-deficient embryos are protected from early
postimplantation embryo loss triggered by maternal exposure to PAHs. Here we
report the results of our investigations into the effects of the identical toxicant
regimen on an inbred genetic background (C57BI/6). This model closely mimics
those conditions in human populations, where women are exposed to chemicals
from cigarette smoke over a long period of time, allowing accumulation of PAHs.
Upon conception, the growing fetal and placental tissues will be exposed to both
metabolized and unaltered PAHs, which have been postulated to exert a variety of
effects on different cell and tissue types (reviewed in [432]), including human
choriocarcinoma cells [433]. Moreover, exposure to PAHs during different stages of
placental development can yield different outcomes. For example, culturing first
trimester placental cells in BaP yielded decreased expression levels of EGF
receptors, whereas Culturing term placental cells resulted in EGF receptor
desensitization [434]. In addition, undifferentiated, proliferative TS cells exposed to
BaP exhibited no changes in levels of cytochrome P450 1A1, whereas expression of
this xenobiotic-metabolizing enzyme was induced in differentiating TS cells [435].
192
In the present study, maternal exposure to PAHs prior to conception caused
fetal intrauterine growth restriction in C57BI/6 dams, as evidenced by reduced fetal
weight and length. Evaluation of two-dimensional placental sections revealed
morphological changes in the labyrinth that included dilatation of the maternal and
fetal vasculature and decreased amounts of collagen at the chorionic plate and
along the large chorionic vessels. The alterations in the labyrinthine
microvasculature were confirmed by SEM of fetal and maternal corrosion casts,
which displayed larger, engorged vessels or blood spaces, irregular anastomoses
and a greater degree of vascular branching and tortuosity. Interestingly, these
changes are strikingly similar to those reported in casts of fetal capillaries from term
placental cotyledons of smoking mothers, which included increased capillary
tortuoisty, density and branching [436]. Finally, thickening of the interhemal distance
and defective labyrinthine vascular remodeling have been reported in dioxin-
exposed rat placentae [437]. Thus, the observed changes in placental vascular
architecture of women smokers may be mediated by the action of PAHs, as
maternal administration of these compounds in our murine model resulted in a
similar vascular phenotype.
The observed changes in vascular structure may be due, in part, to the
effects of PAHs on the extracellular matrix, which we have shown to be affected in
the placentae from exposed dams. Previous reports have shown that cultured
smooth muscle cells exposed to BaP or DMBA exhibited reduced secretion of newly
synthesized collagen [438]. In addition, levels of type | and III procollagen,
accompanied by increased MMP expression, have been reported in skin fibroblasts
193
cultured with tobacco smoke extract [439, 440]. It is possible that in PAH-exposed
murine placentae, expression and/or maintenance of the extracellular matrix proteins
could facilitate the observed changes in vascular architecture. The significant
decreases in arterial surface area and volume obtained from PAH-exposed
placentae, coupled with the reduced diameters of both umbilical vessels likely have
an impact on placental blood flow and/or maternal-fetal exchange. Therefore,
alterations in vascular architecture and blood flow patterns may diminish gas and
nutrient/waste exchange between the mother and the fetus, leading to IUGR.
The importance of cell death during placental development and the
consequences of disrupting this process on fetal and maternal health is highlighted
by gestational diseases such as preeclampsia and IUGR [174, 177]. A clear
difference in cell death rates was observed between the placentae from PAH-
exposed compared with vehicle-exposed dams. A similar reduction in trophoblast
cell death was recently reported in rat placentae treated with dioxin at later
gestational timepoints [437]. Significantly reduced levels of labyrinthine cell death
were observed in PAH-treated placentae, consistent with observations in placentae
from smoking mothers, where decreased apoptosis was observed at term [175,
266]. This decline in the rate of placental cell death is supported by Western
blotting, where decreased levels of cleaved caspase-3, -6, and Bax, were observed
in PAH-exposed placental lysates. Additionally, PAH treatment up-regulated levels
of the anti-apoptotic protein Xiap, a phenomenon previously reported in the placenta
of women smokers [175]. Interestingly, while Bax levels were significantly lower in
placentae from PAH-treated dams, expression levels of FasL were significantly
194
higher. Previous reports have shown that FasL is increased in endothelial cells after
exposure to cigarette smoke extract [430] or ischemia-reperfusion injury [429],
resulting in cytoprotection against Fas-expressing cells of the immune system. FasL
is known to be regulated by AhR [428] and upregulation of this molecule could
explain the decreased cell death rates observed in PAH-exposed placentae.
Furthermore, increased expression of FasL may be a link to why cigarette smokers
have some protection against preeclampsia, where FasL has been shown to be
down-regulated [114]. Lastly, the significant decrease in decidual cell death may
contribute to the observed fetal growth restriction, as apoptosis has been shown to
be involved in remodelling the maternal spiral arteries [192, 441] and perturbations
in this process have been associated with IUGR (reviewed in [189]).
Chronic or acute exposure to ligand in vivo can readily alter expression and
activity levels of ANR [442]. In our model of pre-pregnancy exposure to PAHs,
placental AhR was activated, as evidenced by increased expression levels of p53
and p21, downstream targets of ANR; however, it is presently unknown whether AhR
is activated in the placentae of women smokers. The effects of persistent ANR
stimulation, as evidenced by transgenic mice expressing a constitutively active AhR,
include a reduced life span and the presence of gastric tumours [304]. Acute PAH
exposure typically leads to downregulation of AhR protein by proteasomal
degradation in vitro and in vivo [442, 443]; however, chronic exposure appears to
send the system into a balanced steady state of AhR transcription and degradation
in vivo [442]. In addition with altered levels of transcription, ANR binding affinity is
differentially affected by either acute or chronic doses of dioxin in vivo [444]. It has
195
been proposed that AhR is degraded to regulate the amount of activated AhR and
thus maintain appropriate levels of Arnt for Arnt-dependent pathways [443, 445].
Alterations in labyrinthine cell death were not observed in PAH-exposed AhR-
deficient fetuses — which were also rescued from the IUGR phenotype — highlighting
that PAHs are responsible for this decreased apoptosis in the labyrinth, which
appears to be mediated through the AhR pathway. Moreover, it appears that cell
death has an important physiological function in the labyrinth, likely contributing to
vascular remodeling and allowing optimal cell turnover for this metabolically active
organ. On the contrary, AhR deficiency did not rescue the increased cell death rates
observed in the CP cells, suggesting that while AnR mediates death in the labyrinth,
another cell death pathway may be utilized in the CP. In addition to the observed
collagen deficiencies in PAH-exposed placentae, the increased numbers of TUNEL-
positive, CP cells may be contributing factors to the higher incidence of premature
delivery and premature rupture of the membranes in smoking mothers [446, 447].
In light of the extensive variability in reported phenotypes from both in vivo
and in vitro studies utilizing placentae obtained from smoking mothers, the results of
the present study further illustrate the necessity of considering the genetic context of
observed phenotypes. This is underscored by the fact that only a small proportion of
smokers exhibit !UGR, which has been associated with maternal genotype [126,
403]. We previously reported that ICR dams administered chronic doses of PAHs
prior to conception exhibited a higher resorption rate than those exposed to vehicle
(Figure 4.16a and [425]); however, placental and fetal weights did not differ between
the two groups (Figure 4.16b). Here, we have shown that PAH-exposed C57BI/6
Proportion
of re
sorb
ed
Weig
ht
(g)
embryos
per
litt
er
C57BI/6 d15.5 Fetal and Placental Weights
p<0.001
an
Fetal Weight
0.5
0.45 0.4 0 Vehicle
0.35 m@ PAH-exposed 0.3 0.25
0.2
0.15
0.1
0.05 |__|n=62
Placental Weight
C57BI/6 Resorption Rate (d15.5)
0.3
0.25
0.2
0.15 |
0.1
0.05
n=11 0
Vehicle
Figure 4.16 Maternal exposure to PAHs prior to conception results in
PAH-exposed
Weight
(g)
Proportion
of resorbed
embryos
per
litt
er
0.6
0.5
0.4
0.3
0.2
0.1
196
ICR d15.5 Fetal and Placental Weights
QO Vehicle
@ PAH-exposed
al
0.4
0.35
0.3
0.25
0.2
0.15
0.1
0.05
Placenta Fetus
ICR Resorption Rate (d7.5-d12.5)
I
n=15
p<0.001
Vehicle PAH-exposed
increased resorption rates in ICR dams and IUGR in C57BI/6 dams. A. Graph
depicts significantly increased resorption rates (d7.5-d12.5) in ICR dams after PAH
treatment. B. Graph demonstrates the lack of effect of PAH treatment on d15.5
placental and fetal weights in ICR dams. C. Graph depicts the significant reduction
in d15.5 fetal weight in CS7BI/6 mice after PAH treatment, while (D) depicts the
similar resorption rates seen in PAH-exposed, compared with vehicle-exposed
C57BI/6 dams. Bars represent average values + SE and values of significant
statistical difference are shown with the corresponding p value (Student’s t-test).
197
dams yielded growth-restricted fetuses (Figure 4.16c), but no difference in resorption
rate (4.16d), compared with dams exposed to oil. Furthermore, the majority of these
mice were injected at the same time and with the same formulation, in addition to
being housed in the same room, considerably reducing the number of variables
between the groups. Lastly, AhA-deficiency has been shown to rescue KO fetuses
from PAH-induced IUGR. This receptor is notoriously susceptible to genetic
background, with several polymorphisms in both the promoter and coding regions of
the AhR gene in mice and humans [442, 448]. Such genetic variability will alter
levels of ANR expression and activity, vastly altering phenotypic outcome.
While the primary route of PAH exposure in humans is through tobacco
smoke, the results of these experiments underscore the need to assess the effects
of these compounds through exposure to environmental pollution. Both
epidemiological and clinical studies human populations have reported numerous
deleterious reproductive outcomes due to compounds such as BaP, dioxins,
polychlorinated biphenyls (PCBs) and particulate matter that is found in air, soil and
water (reviewed in [251, 252, 449]). A pivotal study was conducted in the Czech
Republic, which demonstrated the association between environmental pollution and
neonatal mortality [450]. This was followed by several several studies in the USA
and China, where regions considered to have high levels of pollution were linked to
low birth weight, sudden infant death syndrome and neonatal mortality [451, 452].
In addition to chronic exposure to pollutants, disasters such as the terrorist attacks
and subsequent collapse of the buildings of the World Trade Centre (WTC) in New
York on September 11", 2001, can result in acute exposure to compounds such as
198
PAHs, PCBs and heavy metals [453, 454]. Studies of mothers living in close
proximity to the WTC at the time of the attacks revealed an increased incidence of
DNA adduct formation in maternal and fetal white blood cells [455] that was
associated with BaP exposure [456]. Lastly, a similar study revealed that neonates
born to mothers exposed to the various pollutants in the aftermath of the WTC
attacks, exhibited reduced birth weight, length and head circumference [457]. In
light of such profound effects on female reproduction and neonatal outcome, the
murine model of PAH exposure used in these studies would also prove useful in
determining the effects of acute exposure to environmental pollution.
Conclusions
The present study utilizes an animal model of PAH exposure which mimics
the levels seen in human cigarette smokers. C57BI/6 dams chronically exposed to
PAHs prior to conception resulted in aberrant vascularization of both the labyrinthine
and large vessels of the placenta at d15.5, and fetal growth restriction. Histological
sections and corrosion casting of both the maternal and fetal vessels revealed
dilatations and disorganization of the microvasculature of PAH-exposed placentae.
In addition, fetal arterial surface area and volume were significantly diminished, as
determined by microCT, and the umbilical vessels of fetuses from PAH-exposed
dams exhibited decreased diameters. Placentae from mice treated with PAHs
exhibited altered cell death rates, compared with those from control mice,
demonstrating reductions in the labyrinthine region and increases in the CP. AhR
199
deficiency rescued the IUGR phenotype and returned the labyrinthine cell death rate
to control levels; however, it did not affect cell death in the CP. It is concluded PAH
exposure prior to conception results in altered placental vascularization and cell
death patterns that ultimately lead to IUGR.
201
CHAPTER 5: SUMMARY AND GLOBAL CONCLUSIONS
Apoptosis is a required event during metazoan development, required for the
development, differentiation and sculpting of organs, in addition to its role in cell and
tissue homeostasis. Moreover, cell death enables the renewal of old cells,
supporting appropriate cell turnover, while at the same time, preventing injury to
neighbouring, healthy cells. Dysregulation of the apoptotic process can lead to a
diseased state, whereby inhibition of cell death results in the accumulation of
unwanted cells and the potential for subsequent tumourigenesis. Alternatively,
acceleration of the cell death programme can lead to degenerative disorders.
Exposure to PAHs has been previously shown trigger cell death signalling, resulting
in the activation of the apoptotic pathway and leading to the demise of crucial cell
types, such as immune cells and lung epithelium. During pregnancy, exposure to
cigarette smoke — which is the primary route of PAH exposure in humans — has
been associated with reduced fertility and a high miscarriage rate. On the other
hand, PAH exposure has also been implicated in impeding the cell death process,
resulting in tumour formation. A number of different placental phenotypes have
been reported in human conceptuses from smoking mothers, including altered cell
death rates, hyperplasia and premature rupture of the membranes. In addition,
exposure to cigarette smoke during pregnancy is now causally associated with
IUGR, a fetal outcome linked to altered placental cell death rates. While cell death
in the human placenta has been recognized as a physiological event, virtually no
studies have been done on the mouse placenta. In this thesis, | have described
normal cell death patterns and expression of apoptosis-related proteins during
202
mouse placental development and have outlined the consequences of Bax-
deficiency. Furthermore, maternal treatment with PAHs was used as a trigger to
alter cell death rates in outbred, inbred and genetically modified strains of mice.
In chapter two, | reported the results of a systematic and quantitative
examination into cell death patterns in both ICR and C57BI//6 placentae, over
gestation. In addition, the effects of Bax deficiency on murine placentation and its
effects on the fetus were investigated. Over gestation, ICR and C57BI/6 placentae
exhibited TUNEL-positive patterns similar to those observed in human placentae,
with scattered, infrequent death observed in early placentae, which increased
towards term. The most striking observation was the organized pattern of cell death
surrounding the vessels of the labyrinth at mid-gestation, with an apparent role in
remodeling the vasculature of this region. Organized, classically apoptotic cell death
was also detected in TGCs, which are almost completely eliminated towards the end
of gestation. In addition, massive aponecrotic death of intermingled GlyT and
maternal decidual cells was observed in the last quarter of pregnancy. While cell
death patterns were similar for both strains of placentae examined, C57BI/6
placentae typically demonstrated greater numbers of dead cells in almost all regions,
starting at d13.5. Moreover, the unique Parp-1 cleavage profile and TUNEL-staining
patterns observed in the mouse placenta indicate that both classical and non-
classical cell death pathways are functioning within this organ. Lastly, pro-apoptotic
Bax protein immunolocalized to a subset of TGCs and to cells within the labyrinth,
revealing a role for Bax in programmed cell death of this trophoblast cell sub-type.
In addition, Bax deficiency in the mouse placenta resulted in an altered labyrinthine
203
architecture, including fetal capillary dilatation, leading to fetal IUGR. Only recently
has a functional link between cell death and placental vasculogenesis been reported
in human placenta [318] and the studies herein are the first systemic investigations
into murine placental cell death patterns, revealing its crucial function in placental
vascularization and trophoblast turnover.
The observed defects in Bax-deficient placentae — which included decreased
rates of TGC death and dilatation of the fetal capillaries in the labyrinth — and its
possible effect on the fetus have not been previously described; however, the effects
of Bax deficiency in a number of adult tissues have been rigorously studied. This is
not an uncommon occurrence in the field of gene knockout mouse characterization,
as the placenta is an often neglected organ during these investigations, especially
when viable young are born. Therefore, these studies highlight the need to re-visit
previously constructed, gene-targetted knockout mice and examine the effects of
gene deficiencies on the placenta. This opens up numerous avenues of exploration
into placental biology and can contribute to resolving troublesome issues
surrounding human placentation, ultimately leading to improved fetal and maternal
health.
Apoptosis has been shown to play a critical role during vascular remodelling
and cardiovascular development [458, 459], but the underlying cellular mechanisms
involved remain unclear [460, 461]. Recent studies have demonstrated that cell
death is essential for cardiac outflow tract development in both birds [458] and mice
[462], and contributes to pharyngeal arch artery remodelling during murine
embryogenesis [88]. In the adult, apoptosis has been shown to be essential for re-
204
vascularizing the lung in an animal model of ischemia-induced pulmonary injury
[463]. During human placentation, apoptosis has been shown to have a crucial role
in placental morphogenesis, facilitating implantation, maternal spiral artery
remodelling and cytotrophoblast differentiation [111, 174]. Thus far, only one report
has implicated cell death during normal placental vascularization in humans [318];
however, dysregulation of this process in vascular tissues has been fairly well
studied in a number of different systems. Pulmonary hypertension in congenital
heart disease has been linked to defects in the apoptotic programme [464], and the
combined effects of augmented proliferation and unscheduled cell death contribute
to cardiac and renal hypertension [465]. Additionally, disruption of death signalling
pathways in endothelial cells by Bcl-2 overexpression or caspase inhibition impaired
the formation of vascular-like structures in in vitro [466] and in vivo angiogenesis
assays [467], with both initiator caspase-8 and executioner caspase-3 implicated in
this process. Lastly, activation of the cell death pathway has been described to be a
critical event during melanoma mimicry of vasculogenesis [468].
In chapter three, it was shown that chronic, maternal exposure of ICR mice to
PAHs prior to conception resulted in murine embryonic cell death, acting as a
potential mechanism underlying cigarette-smoking-induced pregnancy loss. Cell
death was preceded by increases in Bax, activation of caspase-3 and decreased
litter size. Moreover, the post-implantation embryonic sex ratio was altered in PAH-
exposed dams, with a greater number of male embryos surviving treatment than
female embryos. The observed embryonic loss could not be prevented by the
disruption of Hrk, but was diminished in embryos lacking Bax. These studies
205
revealed that exposure of early embryos to PAHs reduced the allocation of cells to
the embryonic and placental lineages by inducing apoptosis in a Bax-dependent
manner, thus compromising the developmental potential of exposed embryos.
In chapter four of this thesis, chronic maternal exposure of C57BI/6 mice to
PAHs prior to conception resulted in IUGR in d15.5 fetuses. Furthermore, both
histological and structural adaptations were observed in the placental vasculature of
PAH-exposed dams, with significant reductions in arterial surface area and volume
of the fetal placental vasculature. This altered vascularization was accompanied by
reduced labyrinthine and increased CP cell death rates. As PAHs are known ligands
of AhR, it was hypothesized that embryos deficient in this xenobiotic sensor would
be unaffected by PAH exposure. Indeed, AhA-deficient fetuses were rescued from
PAH-induced growth restriction and exhibited no changes in the labyrinthine cell
death rate. The results of this investigation suggest that chronic exposure to PAHs
is a contributing factor to the development of IUGR in human smokers and
implicated AhR in mediating the biological actions of these compounds.
The studies described in chapters three and four of this thesis contribute to
the growing body of knowledge involving the effects of PAH exposure on pregnancy
and placentation. Spontaneous abortion, reduced fertility rates and IUGR are
manifested in human smokers [253] and were observed in these studies in dams
exposed to PAHs, chemical components found in cigarettes. Thus, these results
recaptiulate many physiological events triggered by tobacco smoke exposure in
humans and further support the usefulness of the mouse as a model for human
placentation.
206
The effects of PAH exposure on a number of different cell and tissue types
have been rigorously studied, leading to the conclusion that PAHs can exert
opposite effects on the cell death pathway [426, 469, 470]. This appears to hold true
in C57BIV/6 placentae, where labyrinthine and decidual cells appeared resistant and
CP cells appeared susceptible to PAH-induced death. Additionally, the two different
Strains of mice produced varying phenotypes upon PAH exposure, corroborating
preceding reports that the AhR gene is highly polymorphic, with distinct biological
effects attributed to genetic background [448]. While ICR dams exposed to PAHs
exhibited higher rates of resorption, this was not evident in C57BI/6 dams. On the
other hand, PAH treatment of C57BI/6 dams yielded growth-restricted fetuses, a
condition not apparent in ICR fetuses. Moreover, AnR may be responsible for
producing these diverse outcomes, as PAH-exposed ICR embryos exhibited higher
levels of ANR and its downstream target, Bax, and AhA-deficient fetuses were
protected from PAH-induced growth restriction. Lastly, the disparity in response to
PAHs between the two strains of mice offer yet another caveat regarding the effects
of genetic background when comparing in vivo murine data between strains.
208
CHAPTER 6: FUTURE DIRECTIONS
Bax as a mediator of trophoblast cell differentiation
Herein, | have described that Bax-deficient placentae exhibit defects in TGC
death and in labyrinthine vascular architecture. Bax is a pro-apoptotic protein that
localizes to TGC in the mouse placenta and functions in mediating the demise of this
trophoblast cell sub-type. Interestingly, Bax expression was also detected in the
labyrinth region and appeared to localize to both the endothelial and syncytial layers;
however, whether Bax immunolocalizes to the ST, or to the endothelium, or both,
was difficult to ascertain. Since the cell death pathway has been shown to function
in ST differentiation [89, 104], it is possible that Bax is involved in this process.
Therefore, precise localization of this protein needs to be determined. This could be
more firmly established by immunohistochemical double- or triple-labelling studies
using anti-Bax, anti-cytokeratin (a trophoblast marker) and/or anti-CD31 (an
endothelial marker); however, this may prove difficult as the mouse placenta
contains a great deal of autofluorescence. In addition, ultra-thin tissue sections (i.e.
~50-100 nm) may be required to definitively identify Bax expression patterns in these
cells. Quantitative RT-PCR studies are currently underway, using cDNA obtained
from both Bax WT and KO labyrinthine tissue, to determine whether Bax deficiency
alters gene expression of trophoblast differentiation markers. In parallel to these
studies, in vitro trophoblast stem (TS) studies could be conducted, exposing these
cells to ST-differentiating cell culture conditions [471], followed by gene expression
analyses, including qRT-PCR and Western blotting. If these experiments yield Bax
expression in ST cells, then derivation of Bax WT and KO trophoblast stem cell lines
209
could be considered. Currently, Bax-deficient mice are on mixed C57BI/6
background and would require back-crossing to a 129 background in order to
efficiently derive TS cell lines. Production of Bax WT and KO TS cells would provide
an in vitro model of trophoblast differentiation, to be subsequently analyzed for a
variety of genetic markers of trophoblast cell differentiation.
While we were able to establish that Bax mediates death in a subset of TGC,
analysis of TUNEL patterns in the other placental regions (i.e. labyrinth, junctional
zone, CP) are ongoing and will provide a more comprehensive overview of cell
death patterns and rates in Bax-deficient placentae. In addition, since a number of
dying Bax KO TGCs appeared necrotic and the activation of this cell death pathway
has been previously demonstrated in Bax-deficient MEFs [74], this phenotype
should be further evaluated and quantified in Bax KO placentae. Again, analysis of
TS cell cultures under undifferentiating and diffierentiating conditions and subjected
to a variety of cell death stimuli would be useful in determining gene expression
patterns of cell death markers. We have previously established that expression
levels of Bax and various caspases are upregulated in TS cells under culture
conditions differentiating towards a TGC fate (Figure 6.1) [472] and it is possible that
Bax deficiency may alter the differentiation programme of this trophoblast cell
subtype. Such information would be valuable in supporting the in vivo data
described in this thesis. Lastly, transmission electron microscopy (TEM) would be
useful in evaluating the ultrastructure of Bax KO placentae, including the interhemal
distance and TGC cellular and nuclear morphology.
210
Figure 6.1 Cell death markers in trophoblast stem cells cultured under
differentiating conditions over time. A. Western blot demonstrating increased
Bax expression in TS cells cultured under differentiating conditions for 48 hours.
Blot was stripped and re-probed with anti-B-actin antibodies as a control for protein
loading. B. Graphs depicting cleavage profiles of caspase-3, -6 and -9 in TS cells
cultured under differentiating conditions over time. Bars represent average values
+SE.
Dens
itom
etri
c ratio
of
cleaved
casp
ase:
tota
l caspase
211
TS cells cultured 48 hrs:
Bax
(3-actin
Undifferentiating Differentiating conditions conditions
Expression levels of cleaved caspases in TS cells under differentiating conditions over time
Wi Cleaved:total caspase-3
@ Cleaved:total caspase-6
Bf. Cleaved:total caspase-9
do d2 d4 dé
Days of TS cell culture.under differentiating. conditions
Figure 6.1
212
immune-mediated rejection of embryonic tissues in PAH-exposed dams
Numerous reports indicate that while high levels of PAHs are
immunosuppressive by triggering apoptosis in various types of immune cells [426,
473], low-level exposure to PAHs can stimulate the immune system [474, 475],
potentially resulting in pathologies such as asthma and autoimmune disorders. The
most abundant immune cell type in both the human and rodent placenta is the
uterine natural killer (UNK) cell, residing mainly in the maternal decidua, with
functions in maternal spiral artery remodelling, cytokine release and, it is believed,
maternal recognition of the “foreign” placental cells. While the physiological roles of
uNK cells are somewhat apparent, the pathways of activation and the mechanisms
by which cytolysis is inhibited, are unclear.
An initial pilot study investigating the extent of uNK infiltration into the
maternal decidua revealed that d9.5 ICR placentae exposed to PAHs exhibit greater
numbers of uNK cells compared with placentae exposed to vehicle (Figure 6.2).
These numbers remain high until approximately d12.5, when numbers fall back to
similar values obtained from control placentae. It is uncertain whether these cells
are acting to suppress or assist the invasion of placental trophoblast cells, as it is
believed uNK cells may be involved in both processes [319, 476, 477]. Further
investigations have revealed that FasL expression — a molecule which protects
fetally-derived placental cells from the maternal immune system — is upregulated in
PAH-exposed, ICR placentae, suggesting a failed attempt to protect the fetal
trophoblast from a PAH-induced, hyper-stimulated maternal immune system.
213
Figure 6.2 Polycyclic aromatic hydrocarbon treatment in ICR dams alters
levels of uNK cells in early placental decidua. Histomicrographs depict d9.5-
d12.5 placental sections from dams exposed to vehicle and PAHs. Histochemistry
using Dolichos biflorus lectin was used as a marker of murine uNK cells and
sections were counter-stained with hematoxylin. The population of maternal uNK
cells are upregulated in d9.5 and d10.5 PAH-exposed placentae, which is
subsequently down-regulated by d12.5.
215
A proposed study would involve investigating the spontaneous resorption
phenotype observed in PAH-exposed ICR females, focusing on the proliferation and
activation status of placental immune cells. It would also be advantageous to
ascertain whether maternal factors, embryonic factors, or both, are responsible for
recruiting and activating these immune cells. To answer this question, embryo
transfer experiments could be implemented. Embryos from PAH-exposed mothers
will be transferred to non-exposed pseudopregnant females and embryos from non-
exposed mothers will be transferred to pseudopregnant PAH-treated females. Both
embryonic-derived and maternal-derived tissues would be evaluated to determine
cell death rates and levels of gene expression in control and PAH-exposed tissues.
The results of such experiments could assist in establishing the role of molecular
pathways involved in maternally-mediated spontaneous abortion and would help
further the understanding of the impact of cigarette smoking on female reproductive
immunology. Moreover, the results of such a study would support the argument that
PAH-exposure, or exposure to cigarette smoke is not just associated with pregnancy
loss, but is a direct cause of pregnancy loss, which extends into a female’s
reproductive health, even after cessation of tobacco use.
Placental phenotype due to AhR deficiency
Studies of ANR- and Arni-deficient mice indicate a defect in vascularization
[298, 478]; however, AhA-deficient placentae have not been thoroughly examined
until now. Previous reports have already shown that AnR KO mice exhibit reduced
post-natal viability and are smaller than their WT counterparts [290]. In the studies
216
described in this thesis, AnR was shown to immunolocalize to the fetal endothelium
of the placenta and AhA-deficient fetuses were resistant to PAH-induced growth
restriction. In dams exposed only to vehicle, d15.5 AhA-deficient fetuses exhibited
reduced weight compared to WT fetuses, indicating a possible placental phenotype.
Examination of AhR KO placental sections revealed alterations in the labyrinthine
architecture, which exhibited dilated and disorganized fetal vessels (Figure 6.3a).
Similar defects of the placental vasculature were seen in Bax-deficient and PAH-
treated, C57BI/6 placentae, both of which also yielded growth-restricted fetuses.
While aberrations in the labyrinthine vasculature of PAH-exposed placentae appear
associated with disturbances in cell death, AnR KO placentae exposed to vehicle
alone exhibited only slightly higher cell death rates compared with AhR WT
placentae. Interestingly, levels of cleaved caspase-3 are elevated in AnR KO
placentae, as determined by Western blotting (Figure 6.3b). Thus, if a greater
number of AnR KO and WT TUNEL-stained sections were evaluated for cell death
rates, this difference might reach statistical significance. Alternatively, the observed
increase in cleaved caspase-3 expression may reflect changes in trophoblast
differentiation, as this classical cell death marker has been implicated in human ST
differentiation [177]. Impaired differentiation and turnover of ST in KO placentae
may be responsible for the observed fetal IUGR, as this trophoblast subtype is
crucial in forming the placental barrier, the site of maternal-fetal exchange.
Therefore, evaluation of trophoblast differentiation markers by (RT-PCR should be
implemented to determine whether trophoblast differentiation pathways are
dysregulated in AhR KO placentae. Again, to provide additional support to in vivo
217
Figure 6.3 AhR-deficient placentae exhibit defective labyrinthine architecture
and altered expression of cell death and vascular markers. A.
Histomicrographs depict d15.5 AhR WT and KO placental sections stained with
Bandeiraea simplicifolia lectin, demarcating fetal blood vessels. B. Graphs depict
densitometric ratios after Western blotting, demonstrating altered gene expression
levels in d15.5 AhR KO placentae compared with AhR WT placentae.
218
d15.5 AhR WT Labyrinth d15.5 AhR KO Labyrinth
BS-l lectin
histochemistry to stain fetal
endothelium
B. Cleaved caspase-3 expression p53 expression
Ba a 4 ws 0.25 8B 04 5 © 8 0.36 p=0.027 £ o2 I 6% 03 fc 2 = 0.25 £0.15 p=0.024 Pe 02 Be o. 2 % 0.15 ga” 2® 0.1 ® 0.05 E 8 0.05 =3 o n=3 aa 0 ¥ oo s 8 AhR WT AhR KO AhR WT AhR KO
PECAM-1 expression Fit-1 expression
ue oO “
0% 0.05 5 1.0 p=0.011
cs 0.04 0.028 B ¢ 08 2 p=0. = 5% 0.03 £§ 06 ES = £3 0.02 Si 0.4 x 5 Ui 0.01 2 0.2
QO 0 n=6 n=6 & 0 n=3
AhR WT AhR KO AhR WT AhR KO
Figure 6.3
219
data, AnR WT and KO trophoblast stem cell lines could be derived; however, since
the current mouse line is on a C57BI/6 background, several generations of back-
crossing to 129 mice would be required, to gain a greater efficiency in TS cell
derivation.
The fetal endothelium of the labyrinth is an important element of the placental
barrier, forming the fourth cellular layer of the interhemal distance. Initial
investigations have yielded alterations in endothelium-specific gene expression in
AhFR-deficient placentae, with decreased levels of PECAM-1 and increased levels of
Fit-1 observed (Figure 6.3b). In addition, consistent with other reports [231, 479], we
have observed p53 immunolocalization in the fetal endothelium of the placental
labyrinth and this protein is down-regulated in KO placentae (Figure 6.3b). Since
AhR has been shown to be involved in p53 regulation [469], AhA-deficiency could
perturb normal endothelial-specific p53 expression and impair placental
vascularization, leading to the observed fetal growth restriction. Finally, tetraploid
aggregation experiments could elucidate whether placental insufficiency is a
mitigating factor in the IUGR and cardiac phenotypes observed in knockout animals.
The studies described in this thesis have elucidated an important
association between cell death and placental vascular remodelling. Since a number
of human gestational pathologies such as preeclampsia and IUGR have been
associated with dysregulated cell death pathways, and the etiologies of these
diseases are still enigmatic, continued investigations into these maladaptations
should be pursued. In addition, the results described herein underscore the
usefulness of the mouse as a model of human placentation and offer a cautionary
220
note in evaluating and describing resulting placental phenotypes in mice of different
genetic backgrounds.
10.
11.
12.
13.
14,
15.
16.
17.
18.
222
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