Up-Regulation and Profibrotic Role of Osteopontin in Human Idiopathic Pulmonary Fibrosis
Role of osteopontin in hepatic neutrophil infiltration during alcoholic steatohepatitis
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Transcript of Role of osteopontin in hepatic neutrophil infiltration during alcoholic steatohepatitis
www.elsevier.com/locate/ytaap
Toxicology and Applied PharmRole of osteopontin in hepatic neutrophil infiltration during
alcoholic steatohepatitisB
Udayan M. Apte, Atrayee Banerjee, Rachel McRee, Elizabeth Wellberg, Shashi K. Ramaiah*
Department of Pathobiology, College of Veterinary Medicine, Texas A&M University, MS4467 College Station, TX 77843-4467, USA
Received 23 June 2004; accepted 7 December 2004
Available online 10 May 2005
Abstract
Alcoholic liver disease (ALD) is a major complication of heavy alcohol (EtOH) drinking and is characterized by three progressive stages
of pathology: steatosis, steatohepatitis, and fibrosis/cirrhosis. Alcoholic steatosis (AS) is the initial stage of ALD and consists of fat
accumulation in the liver accompanied by minimal liver injury. AS is known to render the hepatocytes increasingly sensitive to toxicants such
as bacterial endotoxin (LPS). Alcoholic steatohepatitis (ASH), the second and rate-limiting step in the progression of ALD, is characterized
by hepatic fat accumulation, neutrophil infiltration, and neutrophil-mediated parenchymal injury. However, the pathogenesis of ASH is
poorly defined. It has been theorized that the pathogenesis of ASH involves interaction of increased circulating levels of LPS with
hepatocytes being rendered highly sensitive to LPS due to heavy EtOH consumption. We hypothesize that osteopontin (OPN), a matricellular
protein (MCP), plays an important role in the hepatic neutrophil recruitment due to its enhanced expression during the early phase of ALD
(AS and ASH). To study the role of OPN in the pathogenesis of ASH, we induced AS in male Sprague–Dawley rats by feeding EtOH-
containing Lieber–DeCarli liquid diet for 6 weeks. AS rats experienced extensive fat accumulation and minimal liver injury. Moderate
induction in OPN was observed in AS group. ASH was induced by feeding male Sprague–Dawley rats EtOH-containing Lieber–DeCarli
liquid diet for 6 weeks followed by LPS injection. The ASH rats had substantial neutrophil infiltration, coagulative oncotic necrosis, and
developed higher liver injury. Significant increases in the hepatic and circulating levels of OPN was observed in the ASH rats. Higher levels
of the active, thrombin-cleaved form of OPN in the liver in ASH group correlated remarkably with hepatic neutrophil infiltration. Finally,
correlative studies between OPN and hepatic neutrophil infiltration was corroborated in a simple rat peritoneal model where enhanced
peritoneal fluid neutrophil infiltration was noted in rats injected OPN intraperitoneally. Taken together these data indicate that OPN
expression induced during ASH may play a significant role in the pathogenesis of ASH by stimulating neutrophil transmigration.
D 2004 Elsevier Inc. All rights reserved.
Keywords: Alcohol; Lieber–DeCarli Diet; LPS; Osteopontin; Steatosis; Steatohepatitis
Introduction
Heavy alcohol (EtOH) consumption accounts for more
than 100,000 deaths per year in the US and public health
costs are more than $116 billion per year (NIAAA, 2001).
Alcoholic liver disease (ALD) is a major complication of
heavy EtOH consumption and is characterized by progres-
0041-008X/$ - see front matter D 2004 Elsevier Inc. All rights reserved.
doi:10.1016/j.taap.2004.12.018
i A portion of the data included in this paper were presented in the form
of a platform presentation at the 54th Annual Meeting of Association for
Study of Liver Diseases, Boston, MA, November 2003.
* Corresponding author. Fax: +1 979 845 9972.
E-mail address: [email protected] (S.K. Ramaiah).
sive pathologic stages such as steatosis, steatohepatitis, and
cirrhosis (Diehl, 2002; Lieber and DeCarli, 1982; MacSween
and Burt, 1986; Maher, 2002; Nanji, 2002; Ramaiah et al.,
2004). Alcoholic steatosis (AS), is the initial stage of ALD,
characterized by extensive fat accumulation in the liver
along with mild to moderate liver injury (Galambos, 1972;
MacSween and Burt, 1986; Maher, 2002). Although
considered largely benign, recent investigations have
revealed that AS leaves the hepatocytes highly sensitive to
injury. The mechanisms behind such increased susceptibility
of steatotic liver include cellular changes due to fatty
metamorphosis (Bathgate and Simpson, 2002; Teli et al.,
1995), increased oxidative stress (Baykov et al., 2003;
acology 207 (2005) 25 – 38
Fig. 1. Experimental protocol to develop models of alcoholic steatosis and
steatohepatitis in rats. Male Sprague–Dawley rats (200–220 g) were fed
either a control or EtOH-containing Lieber–DeCarli diet for a period of 6
weeks to induce alcoholic steatosis. To generate a model of alcoholic
steatohepatitis, rats were fed either a control or EtOH-containing Lieber–
DeCarli diet for a period of 6 weeks, and then treated with a single dose
of LPS (10 mg/kg ip in saline) at the end of 6 weeks and sacrificed 24 h
later. Details of the experimental protocol have been described in
Materials and methods.
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–3826
Colell et al., 1998; Yang et al., 1997), decreased regener-
ative ability (Apte et al., 2004), and decreased expression of
peroxisome proliferators-activated receptors (Everett et al.,
2000; Fischer et al., 2003; Galli et al., 2001).
Alcoholic steatohepatitis (ASH), the second progressive
stage in ALD, is a rate-limiting step since a vast majority of
patients with ASH progress to cirrhosis even if they abstain
from drinking (Diehl, 2002; French, 2002; Nanji, 2002).
ASH is characterized by significant fat accumulation in the
liver (steatosis) in combination with neutrophil infiltration
(hepatitis), substantial liver injury, hepatic necrosis, and
apoptosis (Bautista, 2002; Diehl, 2002; Jaeschke, 2002;
Ramaiah et al., 2004). The mechanisms of pathogenesis of
ASH have been extensively studied and include increased
ROS/RNS production (Arteel, 2003; Lieber, 1990; Reinke
et al., 1987), nutritional deficit in the carbohydrates
(Korourian et al., 1999), enhanced pro-inflammatory cyto-
kines and chemokine levels (Hoek and Pastorino, 2002;
Wheeler et al., 2001), and high circulating levels of bacterial
endotoxin or lipopolysaccharide (LPS) in patients with ASH
(Arteel, 2003; Enomoto et al., 1999; Hoek and Pastorino,
2002; Uesugi et al., 2001). Irrespective of the mechanisms
of ASH, one of the most common pathological findings in
human ALD is the presence of neutrophils within the
hepatic parenchyma. However, the precise mechanism for
hepatic neutrophil infiltration and consequent hepatic injury
is not well understood. The role of cellular adhesion
molecules such as selectins, integrins (LFA-1/Mac-1), and
members of Ig gene superfamily (ICAM-1 and 2/VCAM-1)
has been demonstrated (Jaeschke, 2002; Jaeschke and
Smith, 1997a,b) as possible mechanisms for hepatic neutro-
phil infiltration.
In addition to adhesion molecules, recent evidence sug-
gests that a novel class of extracellular proteins called matri-
cellular proteins (MCP) play a critical role in the pathogenesis
of several inflammatory diseases (Francki and Sage, 2001;
Kim et al., 1997; Sodek et al., 2002).MCP are involved in cell
to cell and cell to matrix communication rather than structural
support unlike the ECM proteins. Osteopontin (OPN) is one
of the major MCP involved in cell to matrix communication
and in several inflammatory diseases including glomerular
nephritis (Cotran, 1999; Denhardt et al., 2001; Giachelli and
Steitz, 2000; O’Regan and Berman, 2000), inflammation
during CCl4-induced hepatotoxicity (Kawashima et al.,
1999), in puromycin-induced nephrotoxicity (Denhardt et
al., 2001), and nonalcoholic steatohepatitis (Sahai et al.,
2004). OPN is also a known chemoattractant for macro-
phages and neutrophils (Denhardt et al., 2001). However, the
role of OPN in hepatic neutrophil infiltration during ASH has
not been tested thus far. During ASH, neutrophils migrate to
the liver upon activation by cytokine and chemokine signals.
Once in the hepatic sinusoids they have to under go
transmigration to induce hepatocyte damage (Jaeschke,
2002; Jaeschke and Smith, 1997a,b; Jaeschke et al., 1991).
Transmigration involves movement of neutrophils from
hepatic sinusoids into space of Disse, which is the pseudo-
basement membrane in the liver. Neutrophils express specific
cell surface proteins such as h2 integrins [LFA-1 (CD11a/
CD18) and Mac-1 (CD11b/CD18)] and shed other cell
surface proteins such as L-selectin (CD62L) in response to
cytokine signals during neutrophil transmigration (Jaeschke
and Smith, 1997a,b). The primary objective of this study was
to investigate the role of OPN during steatohepatitis of ALD.
The hypothesized role of increased hepatic production of
OPN during early phase of ALD (AS and ASH) leading to
enhanced neutrophil infiltration in the liver, resulting in
hepatic injury was tested on this study. In the current study,
we examined the role of OPN in the development of ASH in a
rat model and examined the relationship between OPN and
neutrophil infiltration.
Materials and methods
Development of AS and ASH models. Simple models of AS
and ASH were developed based on the previous reports
(Deaciuc et al., 2002; Enomoto et al., 1999). Schematic
representation of the development of AS and ASH models is
shown in Fig. 1. Male Sprague–Dawley rats (220–250 g)
were purchased from Harlan Sprague–Dawley, Houston,
TX, USA, and were housed individually in cages in a
temperature-controlled animal facility with a 12-h light–dark
cycle. Rats were utilized after a 1-week equilibration period.
Development of AS model. Rats were divided into two
groups (n = 12 each), control diet group and experimental
diet group, and fed either control (isocaloric control diet
where the calories were adjusted with maltose-dextrin) or
EtOH-containing (35.5% of total calories) Lieber–DeCarli
diet (Bio-Serv, Frenchtown, NJ, #F1697SP) for a period of
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–38 27
6 weeks. For the first day, rats received plain liquid diet;
next, alcohol-treated rats received liquid diet containing
alcohol to 2% and 4% (w/v), each for 2 days. The 4% alcohol
diet was then continued for 6 weeks. The energy distribution
from the EtOH liquid is as follows: 18% protein, 35% fat,
and either 47% carbohydrate (control group) or 11.5%
carbohydrate (maltose dextrin) and 35.5% EtOH (EtOH-fed
groups). The food consumption was recorded daily and the
control rats were pair-fed according to the food consumption
of EtOH-fed rats. Rats were weighed at the beginning of the
study and weekly thereafter. Calories consumed by each rat
were measured daily. Rats were sacrificed at the end of
6 weeks (n = 4) by CO2 asphyxiation.
Development of ASH model. Following acclimatization,
rats were divided into four groups (n = 6 each group):
control, control + LPS, EtOH, and EtOH + LPS. EtOH and
EtOH + LPS group rats were fed Lieber–DeCarli liquid diet
(Bio-Serv, Frenchtown, NJ, #F1697SP) containing EtOH
(35.5% of total calories) for 6 weeks as described for the AS
model. Control and control + LPS group rats received an
isocaloric control diet where the calories were adjusted with
maltose–dextrin. At the end of 6 weeks, rats from control +
LPS and EtOH + LPS groups were injected with a single
injection of LPS (Escherichia coli 0111:B4, 10 mg/kg ip in
saline). The vehicle controls received an equal volume of
saline. All other rats were sacrificed at 24 h after LPS or
vehicle injection, which was given at the end of 6 weeks of
either control or EtOH containing Lieber–DeCarli diet
feeding. All animals were provided humane care in com-
pliance with the institutional guidelines (ULACC; Univer-
sity Laboratory Animal Care Committee) of Texas A&M
University.
Sample collection and processing. Blood was collected
from the dorsal aorta in heparinized tubes. Twenty micro-
liters of heparinized blood was separated in gas chromatog-
raphy vials (VWR, Bristol, CT) and submitted at an in-
house facility for estimation of blood alcohol content (BAC;
Department of Human Anatomy and Medical Neurobiology
at the Texas A&M Health Sciences Center, College Station,
TX). A fraction of heparinized plasma (approximately 0.5ml)
was employed for estimation of liver transaminase activities,
while the remaining plasma was snap frozen in liquid N2
and stored at �70 -C. Livers were harvested, weighed, and
divided into two parts. Three slices of the large and median
lobes were fixed in 10% neutral buffered formalin, while
remaining liver tissue was snap frozen in liquid N2 and
stored at �70 -C for further analysis.
Evaluation of liver injury. Liver injury was estimated by
plasma transaminase activities (alanine aminotransferase;
ALT and aspartate aminotransferase; AST) and corroborated
by histopathology of H&E-stained liver sections. Plasma
ALT and AST activities were analyzed on Vitros Chemistry
Analyzer (Ortho-Clinical Diagnostics, Raritan, NJ). For
histopathology, 4-AM-thick paraffin-embedded liver sec-
tions were cut and stained with H&E for bright-field
microscopy. Liver sections were evaluated for steatosis,
neutrophil inflammation, necrosis, and apoptosis. Hepatic
steatosis was scored using a system developed for the
intragastric infusion model of ALD as previously described
(Nanji et al., 1989) as follows: steatosis (the percentage of
hepatocytes containing fat) <25%, 1+; <50%, 2+; <75%,
3+; >75%, 4+. To assess the degree of inflammation, the
number of neutrophils per five high power fields was
quantitated from the H&E-stained liver sections. The
pathological alterations were evaluated and confirmed by
a board-certified pathologist.
Plasma endotoxin assay. Plasma endotoxin levels were
measured using a Limulus Amebocyte Lysate Endpoint
Assay Kit (BioWhittaker, Walkersville, MD). Pyrogen-free
procedures were employed throughout the assay. All plasma
samples were brought to room temperature prior to the
assay. The plasma samples were diluted (1:10) with LAL
Reagent water and heated in a 70 -C water bath for 5 min. A
pyrogen-free 96-well microplate was preheated at 37 -C.The standards and samples were then incubated with LAL
for 10 min at 37 -C followed by incubation with substrate
solution for 6 min. The reaction was stopped by adding 25%
acetic acid, and the absorbance was read at 410 nm using a
pyrogen-free microplate reader (Benchmark Plus, Bio-Rad,
Hercules, CA), preheated at 37 -C.
Assessment of apoptotic cells. Apoptotic cell death was
detected by morphological changes on light microscopy,
immunohistochemical localization of activated caspase-3
and by TUNEL assay. Apoptotic cells was visualized and
counted by TUNEL assay using ApopTag detection kit
(Serologicals Corporation, Norcross, GA) according to the
manufacturer’s protocol. Paraffinized liver sections of
samples from AS, ASH, and control groups were used.
Four slides per group per time point were stained and
apoptotic cells identified by dark brown nuclear staining
were counted under light microscope (Olympus BX45;
Olympus, Melville, NY). Apoptotic cells were identified by
dark brown nuclear staining and were quantified under light
microscope (Olympus BX51; Olympus, Melville, NY).
For immunohistochemistry of activated caspase-3, depar-
affinized 4 AM thick formalin-fixed paraffin-embedded
unstained liver sections were treated with 3% solution of
H2O2 in order to quench the endogenous peroxidase
activity. Sections were then incubated with blocking
solution (BioStain Rabbit IgG System, Biomeda, Foster
City, CA) to block nonspecific binding sites. An anti-
activated caspase-3 polyclonal antibody (Abcam, Cam-
bridge, MA, dilution of 1:100) was employed as a primary
antibody. Sections were then treated with a biotinylated anti-
rabbit secondary antibody followed by streptavidin (Bio-
Stain Rabbit IgG System, Biomeda, Foster City, CA). The
color was developed by exposing the peroxidase to
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–3828
diaminobenzidine reagent (Vector Laboratories, Burlin-
game, CA), which forms a brown reaction product. The
sections were then counterstained with Gill’s hematoxylin.
Activated caspase-3 expression was identified by the brown
colored cytoplasmic staining.
Three different approaches were employed to ensure
accurate detection of apoptosis: Firstly, the H&E-stained
sections were reviewed under light microscope for apoptotic
morphology such as condensation of chromatin and
pyknotic nuclei. Secondly, TUNEL staining was performed
and cells with definite nuclear dark brown staining were
quantified and compared with H&E sections. Thirdly,
activated caspase-3 immunohistochemical staining was
performed to visualize the cytoplasmic staining of apoptotic
cells. The results of these approaches were evaluated
simultaneously to quantify the degree of apoptosis in AS
and ASH.
RNA extraction and RT-PCR analysis of OPNmRNA. Total
RNA was extracted from frozen liver tissue after lysis and
homogenization using the RNeasy Midi kit (Quiagen,
Valencia, CA) according to the manufacturer’s protocol.
RNA purity was estimated by agarose gel electrophoresis
and spectrophometry. RT-PCR was carried out using
Titanium One-Step RT-PCR kit (BD Biosciences Clontech,
Palo Alto, CA). The primers employed in the RT-PCR
reaction were as follows: OPN forward-5VTCC AAG GAG
TAT AAG CAG AGG GCC A 3Vand reverse-5VCTC TTA
GGG TCT AGG ACT AGC TTG T-3V. The GAPDH RT-
PCR amplimer set (BD Bioscience Clontech, Palo Alto,
CA) was employed as an internal control. A total of 1 Ag of
total RNA was reverse transcribed to cDNA and further
subjected to PCR reaction at 94 -C for 45 s, 50 -C for 30 s,
and 72 -C for 1.5 min for 35 cycles. The PCR products (600
bp for GAPDH and 200 bp for OPN) were detected by 1%
agarose gel electrophoresis.
Western blot analysis for OPN. Liver cell lysates were
prepared in lysis buffer (1% Triton X-100, 50 mM NaCl, 10
mM Tris, 1 mM EDTA, 1 mM EGTA, 2 mM Na vanadate,
0.2 mM PMSF, 1 mM HEPES, 1 Ag/ml leupeptin, and 1 Ag/ml aprotinin) and protein concentration was estimated using
a Bio-Rad protein assay kit (Bio-Rad, Hercules, CA)
according to the manufacturer’s protocol. Briefly, 100 Agof cell lysate was resolved by electrophoresis on a 12%
sodium dodecyl sulfate (SDS) polyacrylamide gel (100 V,
1.5 h) in a running gel buffer containing 25 mM Tris, pH
8.3, 162 mM glycine, and 0.1% SDS. The samples were
transferred to nylon membrane for 3 h at 500 mA. The
membranes were incubated overnight in a cocktail contain-
ing rabbit polyclonal antibodies against recombinant human
OPN (LF-123 and LF-124, generous gift from Dr. Larry
Fisher, National Institute of Dental and Craniofacial
Research; 1:100 dilution in T-TBS with 0.1% Tween and
2% milk) overnight and subsequently probed with HRP-
conjugated anti-goat secondary antibody for 2 h at room
temperature. LF-123 recognizes the native (uncleaved) form
of OPN (¨68 kDa), while LF-124 recognizes the thrombin-
cleaved form of OPN (30 kDa; Rittling and Feng, 1998).
Final visualization was carried out with the enhanced
chemiluminescence kit (Pierce, Rockfor, IL). GAPDH was
used as an internal control to ensure equal loading of
proteins per well.
Immunohistochemistry. Hepatic OPN expression was
studied by immunohistochemical analysis conducted on
4-AM-thick formalin-fixed paraffin-embedded liver sec-
tions. Briefly deparaffinized 4-AM-thick paraffin-embedded
unstained liver sections were treated with 3% solution of
H2O2 in order to quench the endogenous peroxidase
activity. Antigen retrieval was achieved by citric acid
treatment. Sections were then incubated with 10% horse
serum in PBS to block nonspecific binding sites. An anti-
mouse OPN antibody (American Research Products, dilu-
tion of 1:500) was employed as a primary antibody. This
antibody recognizes both the native and cleaved forms of
OPN. Sections were then treated with a biotinylated rat-
adsorbed anti-mouse secondary antibody followed by
streptavidin (Vectastain Elite ABC Kit, Vector Laboratories,
Burligame, CA). The color was developed by exposing the
peroxidase to diaminobenzidine reagent (Vector Laborato-
ries, Burligame, CA), which forms a brown reaction
product. The sections were then counterstained with Gill’s
hematoxylin. OPN expression was identified by the brown-
colored cytoplasmic staining.
OPN ELISA. Serum levels of OPN in AS, ASH, and
control groups were determined using a commercially
available rat OPN ELISA kit (Assay Designs, Ann Arbor,
MI) according to the manufacturer’s protocol. The kit
utilizes polyclonal antibody to mouse OPN, immobilized
on a microtiter plate to bind the rat OPN in the standards and
sample. A rabbit polyclonal antibody to rat OPN labeled
with HRP is employed as a secondary antibody.
Culture and treatments of Hep G2 cells. To further test
the ability of EtOH and EtOH + LPS to induce OPN
expression and confirm the in vivo findings, 1 � 106 Hep
G2 cells were cultured in DMEM with 10% fetal calf
serum. Cells were then treated with increasing concen-
trations of EtOH (25, 50, 100, and 200 mM EtOH for
24 h). In a separate experiment, cells were treated with
either EtOH alone (100 mM) or EtOH + LPS (200 mM
and 1 Ag/Al, respectively) for 24 h. Following treatment
and incubation, cells were lysed in lysis buffer (1% Triton
X-100, 50 mM NaCl, 10 mM Tris, 1 mM EDTA, 1 mM
EGTA, 2 mM Na vanadate, 0.2 mM PMSF, 1 mM
HEPES, 1 Ag/ml leupeptin, and 1 Ag/ml aprotinin) on ice
and homogenates were prepared. Protein estimation was
carried out using Bio-Rad protein assay reagent (Bio-Rad,
Hercules, CA) and 100 Ag of protein was employed for
Western blotting of OPN as described before.
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–38 29
Cause and effect study to demonstrate the relationship
between OPN and neutrophil infiltration in an experimental
rat peritoneal model. Based on the correlative data
between hepatic neutrophil infiltration and OPN expression,
it is highly likely that OPN is most likely playing a role in
hepatic neutrophilic infiltration during ASH. However, to
confirm the correlative studies, an in vivo experiment was
designed to evaluate the chemotactic role of OPN in a rat
peritonitis model as described by Yao et al. (2003). Male
Sprague–Dawley rats (220–250 g) were allocated to 4
groups (n = 4 in each group). One group of 4 rats were
injected 5 mg of zymosan in 0.2 ml of PBS (pH 7.4) into the
subomental space which served as a positive control for
peritoneal neutrophilic infiltration. This protocol is known
to induce neutrophilic infiltration and peritonitis, 4 h post-
zymosan injection. The second group received a control
solution (0.2 ml of PBS). The third group received 100 Agof OPN in PBS (pH 7.4), and the fourth group received 100
Ag of OPN in thrombin (OPN incubated with thrombin for
30 min at 37 -C yielded cOPN). All solutions were
irradiated under UV to ensure sterility. Rats were then
sacrificed at 4 h post-treatment for evaluation of total WBC
and neutrophil response. Before sacrifice the rats were
injected intraperitoneally with 5 ml of ice-cold sterile PBS
containing 20 U/ml of heparin. The abdomen was massaged
for 2 min and then via a midline abdominal incision, free
fluid was recovered from the peritoneal cavity. This fluid
was pooled before being centrifuged at 1000g for 5 min at
4 -C to separate fluid and cellular components. Supernatants
were removed and evaluated for the numbers of leukocytes
using a Abbott Cell-dyn 3700 hematology analyzer (Abbott
Labs, Abbott Park, IL) and confirmed by Beckman T543
cell counter (Beckman Coulter Inc., Brea, CA). Cytospins of
the peritoneal cells were prepared by centrifugation at 500g
for 5 min and these cytospins were stained using Diff-Quik
and the differential counts were determined by light micro-
scopy. The total number of leukocytes and absolute
neutrophil numbers in the OPN-treated group were com-
pared with the zymosan-treated group and vehicle controls
to determine the chemotactic potential of OPN.
Statistics. Group comparisons were performed using
independent t test. A one-way analysis of variance was
used to determine statistical significance that might exist
between more than two distributions or sample groups.
Statistical analyses were made using SPSS 10.0 software
(SPSS Inc., Chicago, IL). Statistical significance was set at
P � 0.05.
Results
Simple models of alcoholic steatosis and steatohepatitis
EtOH alone administration for 6 weeks resulted in
significant fat accumulation (AS), while EtOH adminis-
tration for 6 weeks followed by LPS injection (10 mg/kg,
ip) resulted in fat accumulation along with neutrophil
infiltration, oncotic necrosis, and apoptosis (see below),
which are characteristic of human ASH. The pathology
noted in both AS and ASH is similar to that noted in
human cases of ALD (Diehl, 2002; MacSween and Burt,
1986; Maher, 2002; Nanji, 2002). Body weight gain of
rats in both AS and ASH group was not different from
the control diet-fed rats (333 T 7 in controls vs. 328 T 15
in EtOH-fed) indicating no nutritional differences between
the rats in AS, ASH, and control groups. The average
blood alcohol content in EtOH-fed rats was 83.65 T16.75 mg/dl.
Liver injury, steatosis, inflammation, oncotic necrosis, and
apoptosis
Liver injury estimated by plasma ALT (Fig. 2A) and
AST activities (Fig. 2B) indicated that rats in AS group
developed minimal to no liver damage. Following LPS
challenge plasma transaminase activities increased signifi-
cantly in the rats in ASH group indicating extensive
hepatocellular injury. The H&E-stained liver sections
corroborated the plasma transaminase activity data with
minimal to none hepatocyte necrosis in AS group (Fig. 3C)
and extensive multifocal neutrophil infiltration, and oncotic
coagulative necrosis in the ASH group (Fig. 3D). There was
no distinct zonality pattern in neutrophil infiltration and
necrosis present. The increase in AST observed in control
rats treated with LPS was minimal and histological sections
corroborated minimal necrosis in control and control + LPS-
treated groups (Figs. 3A and B). Scoring of H&E-stained
liver sections from AS group for steatosis (Fig. 4A) and
ASH group for inflammation (Fig. 4B) suggested extensive
steatosis in the rats with AS and significant neutrophil
inflammation in the ASH group. The control + LPS-treated
rats experienced moderate inflammation. There was a lack of
definite regiospecificity in the distribution of fat, neutrophil
infiltration, and coagulative necrosis in the EtOH + LPS-
treated rats. The histopathological observation of H&E-
stained liver sections corroborated the ALT and AST
activities.
Endotoxin levels
Endotoxin levels were detected in the plasma of control,
control + LPS, EtOH, and EtOH + LPS-treated rats using a
standard limulus amebocyte lysate endpoint assay (Fig. 5).
EtOH treatment alone did not increase circulating levels of
LPS. However, increased endotoxin levels were noted in
control and EtOH-fed rats treated with LPS. There were no
significant differences in the levels of plasma endotoxin
between control + LPS and EtOH + LPS-treated rats,
suggesting that the enhanced liver injury in EtOH + LPS-
treated rats is not due to higher LPS levels alone but may
due to the interaction of EtOH and LPS exposure.
Fig. 2. ALT (A) and AST (B) activities in plasma of rats fed either control
or EtOH-containing Lieber–DeCarli liquid diet for 6 weeks followed by a
single injection of LPS or vehicle as described in Materials and methods.
EtOH + LPS-treated rats exhibited significant increase in liver injury as
demonstrated by elevation in plasma ALT and AST activities. *Value
significantly different than all other groups; ! value significantly different
than respective control group. Data are expressed as mean T SE, P � 0.05.
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–3830
Apoptosis
Early and late apoptotic cell death was detected by
immunohistochemical staining of activated caspase-3 (Fig.
6, upper panels A–D) and TUNEL assay, respectively (Fig.
6, lower panel). Both TUNEL assay (Fig. 6, lower panel)
and activated caspase-3 staining (Fig. 6, upper panel C)
indicated apoptosis in the rats from AS group. LPS
treatment further increased apoptosis in both the control
and EtOH-treated (ASH) rats, but the number of apoptotic
cells was significantly higher in the ASH group (Fig. 6,
lower panel and upper panels B and D).
OPN mRNA and protein expression in steatosis
RT-PCR analysis of OPN indicated extremely low levels
of OPN mRNA expression in the livers of control rats.
However, EtOH treatment for 6 weeks resulted in enhanced
OPN mRNA expression in the livers (Fig. 7A). Correspond-
ing to themRNAdata, EtOH treatment for 6weeks resulted in
significant induction in OPN protein as observed in the livers
of AS group rats by Western blot analysis (Figs. 8A and B)
and immunohistochemistry (Fig. 9). The circulating levels of
OPN did not change after EtOH treatment (Fig. 10).
OPN mRNA and protein expression in steatohepatitis
Based on the functional role of OPN in post-ischemic
macrophage infiltration (Persy et al., 2003), and macrophage
migration into hepatic necrosis (Kawashima et al., 1999), we
hypothesized that OPN is over-expressed in liver to attract
neutrophils. Furthermore, based on the enhanced biologic
activity of processed form (thrombin-cleaved) of OPN, we
measured the cleaved form of OPN and correlated with
neutrophil infiltration. LPS treatment to control and EtOH-
fed rats induced OPN mRNA expression, although EtOH +
LPS rats had slightly higher OPN mRNA (Figs. 7A and B).
Similar induction in both hepatic (Figs. 8 and 9) and plasma
levels (Fig. 9) of OPN were observed. The hepatocytes
surrounding the inflammatory foci stained maximally for
OPN following LPS challenge (Fig. 9D). The OPN expres-
sion was predominantly localized to hepatocytes. Although,
the control diet-fed rats treated with LPS exhibited an
induction in OPN in the liver and plasma, the OPN expression
in the ASH group was maximum and significantly higher
than the control + LPS group. The thrombin-cleaved form of
OPN was higher in the ASH group as compared to control +
LPS and AS group. The extent of hepatic neutrophil
infiltration significantly correlated with the induction of
cleaved form of OPN expression in the liver (R2 = 0.86).
OPN expression in Hep G2 cells
To further test the ability of EtOH and EtOH + LPS to
induce OPN, Hep G2 cells were incubated with increasing
concentrations of EtOH. EtOH induced OPN at 50 mM
concentration, but higher concentrations (100 and 200 mM)
failed to induce further OPN expression (Fig. 11). Hep G2
cells incubated with EtOH + LPS resulted in further
induction of OPN than EtOH alone. These in vitro data
provide additional evidence that OPN is induced following
EtOH and EtOH + LPS exposure.
Cause and effect study to assess OPN-mediated neutrophil
response
An experimental rat zymosan-induced peritonitis model as
described by Yao et al. (2003) was modified to confirm the
correlative data between neutrophil infiltration and OPN
expression in the alcoholic steatohepatitis model. Zymosan
injection intraperitoneally is known to significantly enhance
peritoneal neutrophil accumulation resulting in peritonitis
which was confirmed in our studies (Fig. 12). Zymosan-
induced increases in the peritoneal fluid total WBC count
(>2-fold) and the absolute neutrophil numbers (>50-fold)
were compared with OPN-treated group (Fig. 12). The
increase in total WBC count was contributed mostly by
neutrophils and macrophages. Lymphocytes and mast cell
numbers were not altered between the groups. OPN-treated
group (both uncleaved and cleaved OPN) resulted in a
significant increase (>5000 cells in the uncleaved OPN group
Fig. 3. Representative photomicrographs of H&E sections of rats fed either control or EtOH-containing Lieber–DeCarli liquid diet for 6 weeks followed by a
single ip injection of LPS or vehicle as described in Materials and methods. EtOH feeding for 6 weeks resulted in significant steatosis, while injection of LPS
following EtOH led to steatohepatitis with neutrophil infiltration, oncotic necrosis, and apoptosis. (A) control; (B) control + LPS; (C) EtOH; (D) EtOH + LPS.
Magnification 20�. Block arrows indicate steatotic hepatocytes, arrowheads indicate neutrophil infiltration, and small arrows indicate necrotic hepatocytes.
Fig. 4. Steatosis score (A) and quantitation of neutrophils as an index of
inflammation (B) in the livers of rats fed either control or EtOH-containing
Lieber–DeCarli liquid diet for 6 weeks followed by a single ip injection of
LPS or vehicle. Steatosis was scored according to Nanji et al. as described
in Materials and methods. EtOH feeding resulted in significant steatosis
while LPS injection to EtOH-fed rats led to extensive neutrophil infiltration.
*Value significantly different than all other groups. Data are expressed as
mean T SE, P � 0.05.
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–38 31
and >2000 cells in the cleaved OPN group) in peritoneal total
WBC count and absolute neutrophil numbers (>1500 cells)
compared to the control group. In fact, the total WBC count
and absolute neutrophil number matched the zymosan-
treated group (Fig. 12). The cleaved-OPN-treated group did
not significantly differ in total WBC count and absolute
neutrophil count compared to the uncleaved-OPN group.
These results clearly suggest the involvement of OPN in
neutrophil infiltration and confirm the correlative findings of
OPN induction and neutrophil infiltration in the alcoholic
steatohepatitis model.
Fig. 5. Endotoxin levels in rats fed either control or EtOH-containing
Lieber–DeCarli liquid diet for 6 weeks followed by a single ip injection of
LPS or vehicle as described in Materials and methods. Endotoxin was
measured in the plasma of rats by limulus amebocyte lysate assay.
Fig. 6. Detection of apoptotic cell death by TUNEL assay and immunohistochemical staining of activated caspase-3 in the livers of rats fed either control or
EtOH-containing Lieber–DeCarli liquid diet for 6 weeks followed by a single injection of LPS or vehicle as described in Materials and methods.
Representative photomicrographs (upper panels A–D, magnification 40�) of activated caspase-3 staining and quantitation of apoptotic cells in liver sections
following TUNEL assay (lower panel). Arrows indicate positive activated caspase-3 hepatocyte staining. *Value significantly different than all other groups;! value significantly different than respective control group. Data are expressed as mean T SE, P � 0.05.
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–3832
Taken together, the correlative data and the cause and
effect studies strongly suggest that OPN expression is
induced in the AS and ASH. Furthermore, it appears that
expression of the cleaved form of OPN is enhanced following
LPS treatment with higher levels of cleaved form in the ASH
group.
Discussion
Our results demonstrate significant OPN induction
during initial stages of EtOH exposure and is further
enhanced following LPS administration. The correlation
between hepatic OPN induction and neutrophil infiltration
indicate that an increase in OPN creates a microenvironment
conducive for neutrophil inflammatory response following
heavy EtOH exposure and facilitates neutrophil transmigra-
tion into liver. Correlation studies between OPN and hepatic
neutrophil infiltration is corroborated by the preliminary
cause and effect studies.
The simplified experimental models of AS and ASH are
based on the previous investigations (de la Hall et al., 2001;
Enomoto et al., 1999; Murohisa et al., 2002; Tamai et al.,
2002) utilizing the interaction of chronic EtOH consumption
Fig. 7. OPN mRNA expression in rats fed either control or EtOH-
containing Lieber–DeCarli liquid diet for 6 weeks as followed by a single
ip injection of LPS or vehicle described in Materials and methods. OPN
mRNA detection by RT-PCR (A) and densitometric analysis (B). GAPDH
was employed as an internal control for RT-PCR to ensure equal loading
of RNA.
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–38 33
combined with a single LPS exposure. In our model, we
were able to demonstrate the complete spectrum of
pathology associated with ASH including steatosis, neu-
trophilic (mild mononuclear) inflammation, hepatocyte
oncotic necrosis, and apoptosis. These simple models of
alcoholic steatosis and steatohepatitis are highly reprodu-
cible, perfectly mimic the human ALD, and allows for
detailed mechanistic investigations into neutrophil trans-
migration and consequent liver injury.
The process of hepatic neutrophil infiltration and sub-
sequent liver injury involves endothelial and neutrophil
adhesion molecules (Shi et al., 1996). Adhesion molecules
such as intracellular adhesion molecules-1 (ICAM-1) and
vascular endothelial cell adhesion molecule-1 (VCAM-1)
present on hepatocytes and endothelial cell, respectively,
and LFA-1, Mac-1 (h2 integrins), and VLA-1 (h1 integrins)
on neutrophils play an important role in the extravasation
and cellular adhesion process (Bautista, 1997; Jaeschke,
2002; Jaeschke and Smith, 1997a,b; Jaeschke et al., 1991).
Nevertheless, it is clear that the cellular adhesion molecules
alone are not enough for neutrophil extravasation (Jaeschke,
2002). Based on our studies, it appears that OPN is an
important intra-hepatic signaling molecule in the develop-
ment of ASH (Fig. 13).
OPN is a secreted glycoprotein and has been well studied
in inflammatory diseases such as glomerular nephritis
(O’Regan and Berman, 2000), nonalcoholic steatohepatitis
(Sahai et al., 2004), cell-mediated immunity, and granuloma
formation (Giachelli and Steitz, 2000), ischemic injury, and
CCl4-mediated liver injury (Kawashima et al., 1999). OPN
has been shown as a chemotractant for macrophages and
neutrophils both in in vitro assays and in vivo experimental
conditions (Davis and Bayless, 2002). OPN has an RGD
domain that binds to avh3 integrins and mediates its cellular
effects (Bayless and Davis, 2001; Denhardt et al., 2001;
Smith et al., 1998). Furthermore, OPN is further cleaved by
thrombin in a smaller form (¨30 kDa), which has higher
chemotactic potential than the native form of OPN (Denhardt
et al., 2001; Giachelli et al., 1998). The thrombin-mediated
cleavage of OPN reveals a hidden domain on the proteins
(SVVYGLR domain), which possibly interacts with a9h1
integrin on neutrophils (Fig. 13). This interaction of cleaved
form of OPN with a9h1 integrin via SVVYGLR domain is
known to activate lymphocytes and neutrophils (Denhardt
et al., 2001; Giachelli et al., 1998; Yokosaki et al., 1999).
In our study, thrombin-cleaved form of OPN was induced
following EtOH exposure during AS and further induction
is observed after LPS administration in ASH (Fig. 8).
Although cleaved form of OPN correlated with neutrophil
infiltration, the expression of uncleaved native form of OPN
during steatosis is an interesting observation. The reason for
enhanced expression of OPN during AS, at a stage when no
neutrophil infiltration is observed can be attributed to the
lack of expression of the cleaved form of OPN. Thrombin-
cleaved OPN was higher in EtOH + LPS (ASH)-treated rats
as compared to EtOH (AS) alone-treated rats. One
possibility for the enhanced cleaved form of OPN and
consequent neutrophil transmigration during ASH can be
attributed to the higher post-translational modification of
OPN. Similar mechanisms may not be operating during
steatosis and thus may explain the lack of neutrophil
transmigration (Fig. 13). This notion is further supported
by the high correlation between higher thrombin-cleaved
form of OPN and neutrophil infiltration in the ASH group
(R2 = 0.86). This interpretation can be justified by the recent
finding that increased chemotaxis of monocytes by throm-
bin-cleaved form of OPN is demonstrated in murine models
of rheumatoid arthritis generated using LPS (Yamamoto et
al., 2003). The ability of EtOH and EtOH + LPS to induce
hepatic OPN expression was further corroborated in vitro
using HepG2 cells (Fig. 11). There is however a higher
baseline level of OPN expression which can be attributed to
the fact that HepG2 cells are of tumor cells in origin. A
recent report has shown that HepG2 cells constitutively
express OPN and constitutive OPN expression is implicated
in cancer development, progression and metastasis (Zhang
et al., 2004).
Being aware that correlation between OPN expression and
hepatic neutrophil infiltration does not necessarily mean a
causative relationship, an in vivo experiment was designed to
evaluate the chemotactic role of OPN in a model similar to
zymosan-induced rat peritonitis as described by Yao et al.
(2003). Using this model we have now demonstrated the
Fig. 9. Representative photomicrographs of immunohistochemical localization of OPN during alcoholic steatosis and alcoholic steatohepatitis. The arrows point
to the localization of OPNwithin the hepatocytes. Magnification 20�. (A) Control; (B) control + LPS; (C) EtOH (AS); and (D) EtOH + LPS (ASH). Brown color
indicates OPN-positive staining. (For interpretation of the references to colour in this figure legend the reader is referred to the web version of the article.)
Fig. 8. OPN protein expression in rats fed either control or EtOH-containing Lieber–DeCarli liquid diet for 6 weeks as followed by a single ip injection of LPS
or vehicle described in Materials and methods. OPN protein detection by Western blot (A) and densitometric analysis (B). GAPDH was employed as an internal
control for Western blot to ensure equal loading of RNA.
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–3834
Fig. 10. OPN levels in plasma of rats fed either control or EtOH-containing
Lieber–DeCarli liquid diet for 6 weeks followed by a single injection of
LPS or vehicle as described in Materials and methods detected by rat-
specific OPN ELISA kit (Assay Design, Ann Arbor, MI). *Value
significantly different than all other groups; !value significantly different
than respective control group. Data are expressed as mean T SE, P � 0.05.
Fig. 12. A comparison of total WBC count and absolute neutrophil numbers
in the peritoneal fluid of control, zymosan treated, uncleaved OPN (OPN),
and cleaved OPN (cOPN) group. Male SD rats were sacrificed at 4-h post-
treatment and peritoneal fluid was collected for WBC evaluation. *Value
significantly different from the control group. Data are expressed as mean T
SE, P � 0.05.
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–38 35
cause and effect relationship between OPN and neutrophil
infiltration. The OPN-mediated peritoneal neutrophil infiltra-
tion was comparable to the zymosan-induced neutrophilic
peritonitis group which served as a positive control. An
interesting observation in our zymosan-induced peritonitis
study is the higher peritoneal infiltration of monocytes/
macrophages in the OPN administered group. It appears that
OPN has higher affinity towards monocyte/macrophage
chemotaxis than neutrophils. This is not unexpected based
on the literature findings. A study from Kawashima et al.
(1999) have shown that osteopontin is known to act as a
chemokine that can induce hepatic monocyte migration
following carbon tetrachloride intoxication in rats. Although
there are high numbers of peritoneal neutrophil in the OPN-
treated group compared to controls, there is however an
interesting discrepancy between our correlative studies and
Fig. 11. Western blot analysis of OPN expression in Hep G2 cell following
24 h exposure to increasing doses of EtOH (panel A; 25, 50, 100, and 200
mM) and EtOH + LPS (panel B; 200 mM and 1 Ag/Al, respectively).
the cause and effect studies with regards to cleaved OPN and
neutrophil infiltration. Correlative studies in the alcoholic
steatohepatitis model showed high correlation between
higher thrombin cleaved form of OPN and neutrophil
infiltration. However, the cause and effect peritonitis model
did not show enhanced neutrophil numbers in the cleaved
OPN group compared to the uncleaved OPN group. This
discrepancy can be attributed to the insufficient amount of
cleaved OPN injected into the peritoneum. A dose–response
study with cleaved OPN and peritoneal neutrophil infiltration
should address this discrepancy and will be investigated in
our future studies. Clearly, based on the correlative and the
preliminary cause and effect studies, the role of OPN during
hepatic neutrophil infiltration is indicated. We are also
planning OPN knockout studies and OPN neutralizing
antibody intervention experiments to further confirm these
findings and clearly these studies should confirm the
definitive role of OPN in hepatic neutrophil infiltration.
Other possibilities for neutrophil transmigration during
ASH are worthy of investigation. In the present study we
have demonstrated that hepatic apoptosis occurs during AS
and ASH. This is similar to the reported literature findings
that the apoptotic cells appear to correlate well with the
occurrence of ASH (Casey et al., 2001; Deaciuc et al.,
2002). Lawson et al. (1998) have reported that excessive
parenchymal cell apoptosis may be an important signal for
transmigration of neutrophils. However, in the present study,
apoptosis may not be the primary signal for the following
reasons: (1) Although apoptosis was present in the AS and
ASH group, the apoptotic cells were not excessive enough
to overwhelm the macrophage scavenging system to result
in neutrophil migration. (2) The neutrophil migration in the
hepatic parenchyma appears to be around hepatocytes
undergoing oncotic coagulative necrosis and these necrotic
hepatocytes are sharply positive for OPN (Fig. 9). (3) EtOH
Fig. 13. The hypothesized role of OPN in hepatic neutrophil infiltration and features of OPN protein for neutrophil recruitment during steatosis and
steatohepatitis. EtOH and EtOH + LPS treatment result in induction of OPN in the liver. However, in the EtOH + LPS (ASH) group, the thrombin cleaved form
OPN is highly induced, correlating with significant neutrophil infiltration. Hepatic neutrophil infiltration is a consequence of neutrophil sequestration in the
portal vasculature, transmigration, and neutrophil adhesion to hepatocytes. The lack neutrophil infiltration in the EtOH alone group can be attributed to the
absence of thrombin cleavage.
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–3836
alone rats experienced significant apoptosis, however there
was a lack of neutrophil infiltration in that group. Together,
these data suggest that parenchymal cell apoptosis per se did
not result in neutrophil transmigration into the hepatic
parenchyma. Although, in our study the degree of apoptosis
correlated well with ASH, the apoptotic cells as a source of
hepatic OPN is unclear and needs additional investigation.
Other less likely mechanism for neutrophil transmigra-
tion is endotoxemia (Arteel, 2003; Wagner and Roth, 1999).
We noted only mild neutrophil infiltration in the LPS alone
group and marked infiltration in the EtOH + LPS group.
These findings suggest that the neutrophil infiltration is not
solely the result of endotoxemia but possibly a sequel to
EtOH + LPS combination. This is supported by the finding
that the OPN expression was highly induced in the EtOH +
LPS group compared to the LPS-alone group.
In addition to the OPN-mediated neutrophil transmigra-
tion mechanism, the mechanistic basis behind OPN induc-
tion is currently unknown. Based on the enhanced expression
of OPN following LPS challenge in EtOH-treated rats and in
HepG2 cells, it appears that LPS-induced cytokines such as
TNF-a (in vivo) and epidermal growth factor (HepG2 cells)
may be responsible for upregulation of OPN expression
(Pennington et al., 1998; Zhang et al., 2004), although not
tested in this study. In fact, recent studies have shown that
epidermal growth factor and pro-inflammatory cytokines can
upregulate OPN production (Sahai et al., 2004; Zhang et al.,
2004). There is no difference in the OPN mRNA between
LPS alone group and EtOH + LPS group. However, the
EtOH + LPS rats appear to have higher post-translational
cleavage of OPN based on the higher thrombin-cleaved form
of OPN resulting in a higher chemotactic form of OPN. It is
thus possible that LPS treatment results in increased
thrombin-mediated cleavage of OPN. Similar increased
chemotaxis of monocytes by thrombin-cleaved form of
OPN has been demonstrated in murine models of rheumatoid
arthritis generated using LPS (Yamamoto et al., 2003).
In summary, we have identified OPN (native and
thrombin-cleaved form) within the hepatocytes during ASH
rodent model and there appears to be a strong correlation
between cleaved form of OPN and hepatic infiltration. The
correlative findings are corroborated with the preliminary
cause and effect study demonstrated by higher peritoneal
neutrophil infiltration following OPN injection into the
peritoneal cavity. Based on our data, we propose a novel
mechanism for the pathogenesis of ASH (Fig. 13). The
mechanisms by which OPN signals to neutrophils remains to
be studied but based on the previous reports (Denhardt et al.,
2001; Giachelli et al., 1998), it can be speculated that OPN
directly interacts with neutrophils via a9h1 integrins.
Similarly, the role of native and thrombin-cleaved OPN in
neutrophil activation remains to be investigated.
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–38 37
Acknowledgments
Supported by the Center for Environmental and Rural
Health, NIH Seed Grant (NIEHS ES09106), and the Office
of Vice-President for Research Toxicology Seed Grant. The
authors wish to thank Catherine Samway, Clinical Pathol-
ogy technician, for her assistance with peritoneal fluid
analysis.
References
Apte, U.M., McRee, R., Ramaiah, S.K., 2004. Hepatocyte proliferation is
the possible mechanism for the transient decrease in liver injury during
steatosis stage of alcoholic liver disease. Toxicol. Pathol. 32, 567–576.
Arteel, G.E., 2003. Oxidants and antioxidants in alcohol-induced liver
disease. Gastroenterology 24, 778–790.
Bathgate, A.J., Simpson, K.J., 2002. Alcoholic fatty liver. In: Sherman,
D.I.N., Preedy, V., Watson, R.R. (Eds.), EtOH and The Liver:
Mechanisms and Management. Taylor and Francis, London, pp. 3–20.
Bautista, A.P., 1997. Chronic alcohol intoxication induces hepatic injury
through enhanced macrophage inflammatory protein-2 production and
intercellular adhesion molecule-1 expression in the liver. Hepatology
25, 335–342.
Bautista, A.P., 2002. Neutrophilic infiltration in alcoholic hepatitis. Alcohol
27, 17–21.
Baykov, I., Jarvelainen, H., Lindros, K., 2003. l-Cartinite alleviates
alcohol-induced liver damage in rats: role of tumor necrosis factor-
alpha. Alcohol Alcohol. 38, 400–406.
Bayless, K., Davis, G.E., 2001. Identification of dual a4h1 integrin binding
sites within a 38 aminoacid domain in the N-terminal thrombin
fragment of human osteopontin. J. Biol. Chem. 276, 13483–13489.
Casey, C.A., Nanji, A., Cederbaum, A.I., Adachi, M., Takahashi, T., 2001.
Alcoholic liver disease and apoptosis. Alcohol.: Clin. Exp. Res. 25,
49S–53S.
Colell, A., Garcia-Ruiz, C., Miranda, C., Ardite, E., Mari, M., Morales, A.,
Kaplowitz, N., Fernandez-Checa, J.C., 1998. Selective glutathione
depletion of mitochondria by ethanol sensitizes hepatocytes to tumor
necrosis factor. Gastroenterology 115, 1541–1551.
Cotran, R.S., 1999. Tissue repair: cellular growth, fibrosis and
wound healing. In: Cotran, R.S., Kumar, V., Collins, T. (Eds.),
Robbin’s Pathologic Basis of Disease. W.B. Saunders, Philadelphia,
pp. 89–112.
Davis, G., Bayless, K., 2002. Matricryptic integrin binding sites in
osteopontin regulate inflammation. Abstract, 3rd International Confer-
ence on Osteopontin and Related Proteins, San Antonio, TX.
Deaciuc, I.V., Nikolova-Karakashian, M., Fortunato, F., Lee, E.Y., Hill,
D.B., McClain, C.J., 2002. Apoptosis and dysregulated ceramide
metabolism in a murine model of alcohol-enhanced lipopolysaccharide
hepatotoxicity. Alcohol.: Clin. Exp. Res. 24, 1557–1565.
de la Hall, P., Lieber, C.S., DeCarli, L.M., French, S.W., Lindros, K.O.,
Jarvelainen, H., Bode, C., Parlesak, A., Bode, J.C., 2001. Models of
alcoholic liver disease in rodents: a critical evaluation. Alcohol.: Clin.
Exp. Res. 25, 254S–261S.
Denhardt, D.T., Giachelli, C.M., Rittling, S.R., 2001. Role of osteopontin in
cellular signaling and toxicant injury. Annu. Rev. Pharmacol. Toxicol.
41, 723–749.
Diehl, A.M., 2002. Liver disease in alcohol abusers: clinical perspective.
Alcohol 27, 7–11.
Enomoto, N., Yamashita, S., Kono, H., Schemmer, P., Rivera, C.A.,
Enomoto, A., Nishiura, T., Nishimura, T., Brenner, D.A., Thurman,
R.G., 1999. Development of a new, simple rat model of early alcohol-
induced liver injury based on sensitization of Kupffer cells. Hepatology
29, 1680–1689.
Everett, L., Galli, A., Crabb, D., 2000. The role of hepatic peroxisome
proliferator-activated receptors (PPARs) in health and disease. Liver 20,
191–199.
Fischer, M., You, M., Matsumoto, M., Crabb, D.W., 2003. Peroxisome
proliferator-activated receptor alpha (PPARalpha) agonist treatment
reverses PPARalpha dysfunction and abnormalities in hepatic lipid
metabolism in ethanol-fed mice. J. Biol. Chem. 278, 27997–28004.
Francki, A., Sage, E.H., 2001. SPARC and the kidney glomerulus:
matricellular proteins exhibit diverse functions under normal and
pathological conditions. Trends Cardiovasc. Med. 11, 32.
French, S.W., 2002. Alcoholic hepatitis: inflammatory cell-mediated
hepatocellular injury. Alcohol 27, 43–46.
Galambos, J.T., 1972. Natural history of alcoholic hepatitis. Histological
changes. Gastroenterology 63, 1026–1035.
Galli, A., Pinaire, J., Fischer, M., Dorris, R., Crabb, D.W., 2001. The
transcriptional and DNA binding activity of peroxisome proliferator-
activated receptor alpha is inhibited by ethanol metabolism. A novel
mechanism for the development of ethanol-induced fatty liver. J. Biol.
Chem. 276, 68–75.
Giachelli, C.M., Steitz, S., 2000. Osteopontin: a versatile regulator of
inflammation and biomineralization. Matrix Biol. 19, 615–622.
Giachelli, C.M., Lombardi, D., Johnson, R.J., Murry, C.E., Almeida,
M., 1998. Evidence for a role of osteopontin in macrophage
infiltration in response to pathological stimuli in vivo. Am. J. Pathol.
152, 353–358.
Hoek, J.B., Pastorino, J.G., 2002. EtOH, oxidative stress, and cytokine-
induced liver cell injury. Alcohol 27, 63–68.
Jaeschke, H., 2002. Neutrophil-mediated tissue injury in alcoholic hepatitis.
Alcohol 27, 23–27.
Jaeschke, H., Smith, C.W., 1997a. Mechanisms of neutrophil-mediated
parenchymal cell injury. J. Leukocyte Biol. 61, 647–653.
Jaeschke, H., Smith, C.W., 1997b. Cell adhesion and migration: III.
Leukocyte adhesion and transmigration in the liver vasculature. Am.
J. Physiol. 273, G1169–G1173.
Jaeschke, H., Farhood, A., Smith, C.W., 1991. Neutrophil-induced liver cell
injury in endotoxin shock is a CD11b/CD18-dependent mechanism.
Am. J. Physiol. 253, H699–H703.
Kawashima, R., Mochida, S., Matsui, A., YouLuTuZ, Y., Ishikawa, K.,
Toshima, K., Yamanobe, F., Inao, M., Ikeda, H., Ohno, A., Nagoshi,
S., Uede, T., Fujiwara, K., 1999. Expression of osteopontin in
Kupffer cells and hepatic macrophages and stellate cells in rat liver
after carbon tetrachloride intoxication: a possible factor for macro-
phage migration into hepatic necrotic areas. Bichem. Biophys. Res.
Commun. 256, 527–531.
Kim, T.H., Mars, W.M., Stolz, D.B., Petersen, B.E., Michalopoulos, G.K.,
1997. Extracellular matrix remodeling at the early stages of liver
regeneration in the rat. Hepatology 26, 896–904.
Korourian, S., Hakkak, R., Ronis, M.J., Shelnutt, S.R., Waldron, J.,
Ingelman-Sundberg, M., Badger, T.M., 1999. Diet and risk of ethanol-
induced hepatotoxicity: carbohydrate-fat relationships in rats. Toxicol.
Sci. 47, 110–117.
Lawson, J.A., Fisher, M.A., Simmons, C.A., Farhood, A., Jaeschke, H.,
1998. Parenchymal cell apoptosis as a signal for sinusoidal
sequestration and transendothelial migration of neutrophils in murine
models of endotoxin and Fas-antibody-induced liver injury. Hepatol-
ogy 28, 761–767.
Lieber, C.S., 1990. Alcohol metabolism and liver injury. Pharmacol. Ther.
46, 1–41.
Lieber, C.S., DeCarli, L.M., 1982. The feeding of alcohol in liquid diets:
two decades of application and 1982 update. Alcohol.: Clin. Exp. Res.
6, 523–531.
MacSween, R.N., Burt, A.D., 1986. Histological spectrum of alcoholic liver
disease. Semin. Liver Dis. 6, 221–232.
Maher, J.J., 2002. Alcoholic steatosis and steatohepatitis. Semin. Gastro-
intest. Dis. 13, 31–39.
Murohisa, G., Kobayashi, Y., Kawasaki, T., Nakamura, S., Nakamura, H.,
2002. Involvement of platelet-activating factor in hepatic apoptosis
U.M. Apte et al. / Toxicology and Applied Pharmacology 207 (2005) 25–3838
and necrosis in chronic ethanol-fed rats given endotoxin. Liver 22,
394–403.
Nanji, A., 2002. Alcoholic liver disease. In: Zakim, D., Boyer, T.D. (Eds.),
Hepatology, A Text Book of Liver Disease. W.B. Saunders, Philadel-
phia, pp. 839–922.
Nanji, A.A., Mendenhall, C.L., French, S.W., 1989. Beef fat prevents
alcoholic liver disease in the rat. Alcohol.: Clin. Exp. Res. 13, 15–19.
National Institute on Alcohol Abuse and Alcoholism, 2001. Alcohol Alert
51.
O’Regan, A., Berman, J.S., 2000. Osteopontin: a key cytokine in cell-
mediated and granulomatous inflammation. Int. J. Exp. Pathol. 81,
373–390.
Pennington, H.L., Wilce, P.A., Worrall, S., 1998. Chemokine and cell
adhesion molecule mRNA expression and neutrophil infiltration in
lipopolysaccharide-induced hepatitis in ethanol-fed rats. Alcohol.: Clin.
Exp. Res. 22, 1713–1718.
Persy, V.P., Verhulst, A., Ysebaert, D.K., De Greef, K.E., De Broe,
M.E., 2003. Reduced postischemic macrophage infiltration and
interstitial fibrosis in osteopontin knockout mice. Kidney Int. 63,
543–553.
Ramaiah, S.K., Rivera, C., Arteel, G.E., 2004. Early-phase alcoholic liver
disease: an update on animal models, pathology and pathogenesis. Int.
J. Toxicol. 23, 217–231.
Reinke, L.A., Lai, E.K., DuBose, C.M., McCay, P.B., 1987. Reactive free
radical generation in the heart and liver of ethanol-fed rats: correlation
with in vitro radical formation. Proc. Natl. Acad. Sci. U.S.A. 84,
9223–9227.
Rittling, S.R., Feng, F., 1998. Detection of mouse osteopontin by western
blotting. Biochem. Biophys. Res. Commun. 250, 287–292.
Sahai, A., Malladi, P., Melin-Aldana, H., Green, R.M., Whitington, P.F.,
2004. Upregulation of osteopontin expression is involved in the
development of nonalcoholic steatohepatitis in a dietary murine model.
Am. J. Physiol.: Gastrointest. Liver Physiol. 287, 6264–6273.
Shi, J., Fujieda, H., Kokubo, Y., Wake, K., 1996. Apoptosis of neutrophils
and their elimination by Kupffer cells in rat liver. Hepatology 24,
1256–1263.
Smith, L.L., Cheung, H.K., Ling, L.E., Chen, J., Sheppard, D., Pytela, R.,
Giacheli, C.M., 1998. Osteopontin N-terminal domain contains a
cryptic adhesive sequence recognized by a9/h1 integrin. J. Biol. Chem.
271, 28485–28491.
Sodek, J., Zhu, B., Huynh, M.H., Brown, T.J., Ringuette, M., 2002. Novel
functions of the matricellular proteins osteopontin and osteonectin/S-
PARC. Connect. Tissue Res. 43, 308–319.
Tamai, H., Horie, Y., Kato, S., Yokoyama, H., Ishii, H., 2002. Long-term
ethanol feeding enhances susceptibility of the liver to orally
administered lipopolysaccharides in rats. Alcohol.: Clin. Exp. Res.
26, 75S–80S.
Teli, M.R., Day, C.P., Burt, A.D., Bennett, M.K., James, O.F.W., 1995.
Determinants of progression to cirrhosis or fibrosis in pure alcoholic
fatty liver. Lancet 346, 987–990.
Uesugi, T., Yin, M., Bradford, B.U., Wheeler, M.D., Uesugi, T., Froh, M.,
Goyert, S.M., Thurman, R.G., 2001. Toll-like receptor 4 is involved in
the mechanism of early alcohol-induced liver injury in mice.
Hepatology 34, 101–108.
Wagner, J.G., Roth, R.A., 1999. Neutrophil migration during endotoxemia.
J. Leukocyte Biol. 66 (1), 10–24 (Jul.).
Wheeler, M.D., Kono, H., Yin, M., Nakagami, M., Uesugi, T., Arteel, G.E.,
Gabele, E., Rusyn, I., Yamashina, S., Froh, M., Adachi, Y., Iimuro, Y.,
Bradford, B.U., Smutney, O.M., Connor, H.D., Mason, R.P., Goyert,
S.M., Peters, J.M., Gonzalez, F.J., Samulski, R.J., Thurman, R.G., 2001.
The role of Kupffer cell oxidant production in early ethanol-induced
liver disease. Free Radical Biol. Med. 31, 1544–1549.
Yamamoto, N., Sakai, F., Kon, S., Morimoto, J., Kimura, C., Yamazaki, H.,
Okazaki, I., Seki, N., Fujii, T., Uede, T., 2003. Essential role of the
cryptic epitope SLAYGLR within osteopontin in a murine model of
rheumatoid arthritis. J. Clin. Invest. 112, 181–188.
Yang, S.Q., Lin, H.Z., Lane, M.D., Clemens, M., Diehl, A.M., 1997.
Obesity increases sensitivity to endotoxin liver injury: implications for
the pathogenesis of steatohepatitis. Proc. Natl. Acad. Sci. U.S.A. 94,
2557–2562.
Yao, V., McCauley, R., Cooper, D., Platell, C., Hall, J.C., 2003. Myelo-
peroxidase response to peritonitis in an experimental model. ANZ J.
Surg. 73, 1052–1056.
Yokosaki, Y., Matsuura, N., Sasaki, T., Murakami, I., Schneider, H.,
Higashimaya, S., Saitoh, Y., Yomakido, M., Taooka, Y., Sheppard, D.,
1999. The integrin alpha(9)beta(1) binds to a novel recognition
sequence (SVVYGLR) in the thrombin-cleaved amino-terminal frag-
ment of osteopontin. J. Biol. Chem. 274, 36328–36334.
Zhang, G.X., Zhao, Z.Q., Wang, H.D., Hao, B., 2004. Enhancement of
osteopontin expression in HepG2 cells by epidermal growth factor via
phosphatidylinositol 3-kinase signaling pathway. World J. Gasteroen-
terol. 10, 205–208.