Attachment and germination of Entomophaga maimaiga conidia on host and non-host larval cuticle
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Transcript of Attachment and germination of Entomophaga maimaiga conidia on host and non-host larval cuticle
Attachment and germination of Entomophaga maimaiga conidiaon host and non-host larval cuticle
Ann E. Hajek* and Callie C. Eastburn
Department of Entomology, Cornell University, Comstock Hall, Ithaca, NY 14853-0901, USA
Received 15 January 2002; accepted 20 November 2002
Abstract
The lepidopteran-specific fungal pathogen Entomophaga maimaiga is highly virulent against Lymantria dispar (gypsy moth)
larvae, and other members of the family Lymantriidae. Numerous species in the subfamily Cuculliinae (Family Noctuidae) are not
susceptible to E. maimaiga due to the inability of this fungus to penetrate the larval cuticle. Conidial attachment and germination
were compared among five cuculliine species and L. dispar using bioassays and scanning electron microscopy. Although conidia
were showered evenly across larvae during bioassays, on L. dispar conidia were most abundant on segments, where they adhered
well to the cuticle and germinated at high percentages. Conidia on cuculliine cuticles were predominantly found in large, loose
aggregations in intersegmental areas. Few conidia on cuculliine cuticle germinated and scanning electron microscopy revealed a
thick film of mucous enveloping conidia. We hypothesize that the conidia on cuculliines become coated by this film and were only
loosely attached to the larval cuticle. No such film was seen on L. dispar larvae where individual conidia appeared well attached. On
L. dispar larvae many conidia also adhered to setae. To determine if hydrophobicity affected the ability of E. maimaiga conidia to
attach and germinate on a substrate, a goniometer was used to determine relative hydrophobicity of larval cuticles. L. dispar cuticle
was more hydrophobic than cuculliine cuticle, suggesting that a high level of hydrophobicity could be a required characteristic for
hosts. Cuticles from four cuculliine species and L. dispar were sequentially extracted using hexane, chloroform, and methanol.
Conidia were showered onto glass slides coated with the different extracts and germination was quantified. Methanol extracts of
cuculliine cuticle consistently decreased germination, compared to all extracts of L. dispar cuticle. For all L. dispar extracts, the
majority of conidia produced germ tubes, which is a normal prerequisite for cuticular penetration. For the cuculliines, conidia
exposed to hexane and chloroform extracts produced secondary conidia as did all controls, but the conidia exposed to cuculliine
methanol extracts that germinated produced germ tubes. These studies demonstrated that a range of factors act in concert to prevent
E. maimaiga infection of the cuculliine species investigated.
� 2003 Elsevier Science (USA). All rights reserved.
Keywords: Entomopathogenic fungi; Entomophthorales; Germination; Adhesion; Cuticle hydrophobicity; Non-target effects; Biological control
1. Introduction
Insect cuticle forms the first formidable barrier to
pathogens. There are a number of discrete stages leading
to breaching the cuticle, including spore attachment,
spore germination, spore differentiation (with or without
formation of appressoria) and then penetration of the
cuticle by enzymatic and mechanical means (St. Leger,
1991). A diversity of factors have been identified as in-fluencing the activity of conidia at the cuticular level.
Conidia of many species of entomopathogenic fungi arethought to initially attach nonspecifically (Boucias and
Pendland, 1991). The hydrophilic conidia of Entom-
ophthorales are covered by a mucilaginous coat that is
released upon cuticular attachment and is thought to act
as a glue (see Boucias and Pendland, 1991). Surface
hydrophobicity has been associated with adhesion of
plant pathogenic fungi (Kuo and Hoch, 1996; Terhune
and Hoch, 1993). Conidial distribution on host cuticlecan be region specific (e.g., Sosa-Gomez et al., 1997) and
surface topography has been shown to influence growth
of deuteromycetes after adhesion (Boucias and Pend-
land, 1991). Chemical components of the cuticle can also
affect conidial development after adhesion by either
Journal of Invertebrate Pathology 82 (2003) 12–22
Journal ofINVERTEBRATE
PATHOLOGY
www.elsevier.com/locate/yjipa
*Corresponding author. Fax: +1-607-255-0939.
E-mail address: [email protected] (A.E. Hajek).
0022-2011/03/$ - see front matter � 2003 Elsevier Science (USA). All rights reserved.
doi:10.1016/S0022-2011(02)00198-2
causing production of nonpenetrant germ tubes or byinhibiting germination altogether (Boucias and Pend-
land, 1991).
The host range of the entomophthoralean pathogen
Entomophaga maimaiga (Zygomycetes: Entomophtho-
rales) is limited. During laboratory bioassays evaluating
larvae of a diversity of forest-dwelling Lepidoptera,
35.6% of 78 species assayed became infected but only
8.2% of susceptible species were infected at levels > 50%(Hajek et al., 1995). Consistently high levels of infection
were only observed among members of the Lymantrii-
dae, the tussock moth family that includes the principal
host of E. maimaiga, Lymantria dispar (gypsy moth)
(Hajek et al., 1995).
Many species of owlet moths (Noctuidae) inhabit the
same or similar forest habitats as L. dispar. One of the
common subfamilies in the Noctuidae is the Cuculliinae,whose larvae have been referred to as arboreal cut-
worms since they feed off the ground and have few setae.
While earlier instars of cuculliines feed in trees, late in-
stars can also be found on the forest floor. High levels of
infection can occur when late instar L. dispar rest in the
leaf litter (Hajek et al., 2000) or when larvae are caged
on top of the soil (Hajek, 2001). However, only one of
47 larvae of the cuculliine Sunira bicolorago collected inthe leaf litter (Hajek et al., 2000) was infected by E.
maimaiga. Curiously, studies comparing infection by
injection of fungal cells with infection requiring cuticu-
lar penetration had demonstrated that cuculliines were
unique among the many species of Lepidoptera tested
(Hajek et al., 1995). When E. maimaiga cells were in-
jected into the hemocoels of six species of cuculliine
larvae, five species became infected although none ofthese were infected when they were challenged by de-
positing E. maimaiga conidia onto their cuticles.
Based on the results of these bioassays and field
studies, we hypothesized that successful infection of
cuculliine larvae by E. maimaiga is prevented at the
cuticle. We compared attachment and germination of
E. maimaiga conidia on the cuticles of L. dispar and
five cuculliine species. Cuticle hydrophobitities and theeffects of cuticular extracts on conidial germination
were also compared among these species.
2. Materials and methods
2.1. Experimental insects
Lymantria dispar larvae used in this study were ob-
tained as neonates from the USDA, APHIS, Otis
Methods Development Center, Massachusetts. They
were reared on high wheat germ diet (Bell et al., 1981) in
236ml plastic cups at 23 �C, 14:10 (L:D).
Noctuids in the subfamily Cuculliinae, Chaetaglaea
sericea, Eupsilia vinulenta, Sericaglaea signata, S. bi-
colorago, and Xylotype capax, were collected in NewJersey. Adult females of species that overwinter as adults
(S. signata and E. vinulenta) were collected in February
or March, when they mate and the other cuculliine
species were collected in late October or November.
Adult females were collected using sugar baits and if
they had not yet mated, they were confined in outdoor
cages with males. Once mated, females were placed
singly in 200ml glass jars. White paper towels wereprovided for oviposition and honey or maple syrup,
diluted 1:2 with water, was provided for food. Eggs
produced were placed in cups outdoors until hatch or
were placed directly into sleeves slightly before hatching.
Larvae from cups were reared on cuttings until late first
or second instar when they were placed in sleeves on
branches of trees or shrubs. Larvae of C. sericea, E.
vinulenta, S. signata, and X. capax were reared on blackcherry (Prunus serotina) and larvae of S. bicolorago were
fed apple (Pyrus malus). Larvae were removed from
sleeves at the penultimate instar and were subsequently
reared in humid, ventilated plastic containers (10.5 cm
diameter� 13 cm height) at 23 �C, 14:10 (L:D) where
they were provided with fresh host plant foliage until use
in experiments.
2.2. Fungal inoculum and infection methodology
The isolate of E. maimaiga used in this study was
ARSEF 6162 (USDA, ARSEF Agricultural Research
Service Collection of Entomopathogenic Fungal Cul-
tures, Ithaca, NY). Hyphal bodies and naturally oc-
curring protoplasts of E. maimaiga were grown in 95%
Grace�s insect tissue culture media (Gibco-BRL, Gai-thersburg, MD) supplemented with 5% fetal bovine se-
rum (Gibco-BRL) at 20 �C in the dark.
To obtain dense showers of conidia over a relatively
short time period, we infected L. dispar larvae and used
resulting cadavers to produce inoculum. Fourth instars
were injected with 10 ll of 1:0� 105 protoplasts/ml in
Grace�s insect tissue culture media and were then
maintained at 20 �C in the dark until death. Insects weremonitored daily from 4 to 6 days post-injection and then
transferred to 100% RH at 15 �C in the dark to initiate
fungal outgrowth and conidial discharge.
2.3. Larval infection
To deliver a consistent dose within each bioassay,
larvae were inoculated by showering conidia on them astheir containers rotated beneath sporulating cadavers
within a ‘‘showering box.’’ Each showering box con-
sisted of an 11.3 L polyethylene storage container
(Rubbermaid Incorporated, Wooster, OH) in which a
15 cm diameter platform was mounted. The platform
was attached to a 0.75 rpm gear motor powered by a
regulated 13.8V power supply. High humidity was
A.E. Hajek, C.C. Eastburn / Journal of Invertebrate Pathology 82 (2003) 12–22 13
maintained within tightly sealed showering boxesby lining the bottom and sides with moistened paper
towels.
To inoculate larvae, 10–15 cadavers that were dis-
charging conidia were placed dorsal side down on net-
ting covering a platform of 1.2 cm mesh hardware cloth
(15� 15 cm). The hardware cloth was suspended 7–8 cm
above test larvae in the showering box. Conidia from
sporulating cadavers fell through the mesh onto testlarvae that were on the rotating platform directly below.
To prevent larvae from escaping during the conidial
shower, they were placed individually in 29.6ml plastic
cups coated internally with Sigmacote (Sigma Chemical,
St. Louis, MD). Seven larvae at a time could be posi-
tioned in cups beneath sporulating cadavers.
2.4. Conidial attachment and germination studies
Studies of attachment and germination of E.
maimaiga conidia to host versus non-host larval cuticle
used 3 fourth instar L. dispar larvae and 3 non-target
larvae between penultimate and ultimate instars for each
of three replicates for each cuculliine species. For each
replicate, conidia were showered onto test insects for a
4-h period. Insects were then placed singly in 29.6mlplastic cups containing moistened filter paper to create a
100% RH environment and leaves from a host plant for
cuculliines or artificial diet for L. dispar. Lids were
placed on cups and larvae remained in these conditions
for a 12-h germination period. Larvae were then trans-
ferred to new 29.6ml plastic cups containing approxi-
mately 3 g silica gel desiccant; this reduced subsequent
condensation on cadavers that could disrupt conidia onthe cuticle. Larvae with desiccant remained at room
temperature for 20min prior to being frozen at )80 �C.After thawing, conidia on dorsal surfaces of cadavers
were counted at 64� using a dissecting microscope. An
ocular grid (750� 750lm) was used to quantify conidial
density and production of germ tubes for ten grids per
larva. Conidia were not evenly distributed on larvae so
we evaluated conidial density and activity by cuticularregion. However, cuculliine and L. dispar larvae have
very different topography of their bodies so we could not
use the same sampling plan for both. L. dispar larvae
have abundant setae attached to segmental areas and,
on many segments, heavily sclerotized dorsal and lateral
elevations that bear setae, called verrucae. Cuculliine
larvae have few setae and no unusual cuticular topog-
raphy. For each cuculliine, we evaluated conidia in fourintersegmental regions and six areas on segments. For
each L. dispar larva, we evaluated conidia on four ver-
rucae, four regions on segments surrounding the verru-
cae and two intersegmental regions. For all larvae,
conidia on setae within the ocular grids were counted
separately, while counting conidia on segments or ver-
rucae.
2.5. Goniometer studies
Hydrophobicity of larval cuticles was evaluated by
measuring the contact angle that a 1mm diameter
droplet of distilled water made with each surface using
an NRC Contact Goniometer (Model 100-00, Ram�ee-Hart, Mountain Lakes, NJ) (Neumann and Good,
1979). The formula used to determine average contact
angle is: cos�1ððcos h1 þ cos h2Þ=2Þ; h1, the advancingangle and h2, the receding angle (Nishino et al., 1999).
Larval cuticles were prepared by cutting the head off of a
larva with a sharp razor and cutting a 1.5� 2.5 cm sec-
tion of cuticle from the dorsum. Larger internal struc-
tures, e.g., tracheae, were carefully removed and the
cuticle was flattened, cuticle-side up, on hardened glue
and secured at the corners with minuten pins. Removal
of the setae from the cuticle of L. dispar was requiredbefore a reading could be taken because the large sec-
ondary setae either prevented the water from touching
the cuticular surface or burst the water droplets so that
readings could not be obtained. For removal, the distal
ends of secondary setae were gently touched with sticky
tape; this removed secondary setae without disturbing
the cuticle surface. Samples were kept at 100% RH until
readings were conducted, generally within 1 h of prep-aration. Two to six cuticles were quantified for each
species, based on availability of larvae.
2.6. SEM preparation
Larvae were showered with E. maimaiga conidia as
described above, followed by a 12-h germination period.
Cuticles were removed as described for goniometer tests,with care being taken to avoid touching the dorsal sur-
face and to prevent internal fluids from washing over the
dorsal surface. Cuticles were stretched and held in place
using minutens inserted in hardened hot glue on top of a
2.54 cm diameter scanning electron microscopy stub,
sputter-coated with 30 nm gold/palladium and subse-
quently observed using a Hitachi 4500.
2.7. Cuticular extract studies
Late instar larvae of four species of cuculliines (E.
vinulenta, S. signata, S. bicolorago, and X. capax) and L.
dispar were starved for 24 h and then frozen at )80 �C.Due to the difficulty in obtaining large numbers of these
cuculliines, groups of twenty were considered represen-
tative for each species. Twenty larvae were thawed andthen each individual was placed in 15ml quantities of
hexane then chloroform, followed by methanol with 15-s
exposures in each solvent. Hexane extracted only
non-polar lipids, chloroform extracted lipids of greater
polarity and methanol extracted more polar organic
constituents. Extracts were concentrated to 1ml using a
rotary evaporator. Larvae of the different species were
14 A.E. Hajek, C.C. Eastburn / Journal of Invertebrate Pathology 82 (2003) 12–22
similar in size and surface areas of larvae of each specieswere approximately estimated as the surface area of a
cylinder. We determined that by spreading 50 ll of anextract on an 18� 18mm cover slip, we would be ap-
proximating the concentration found on the cuticle of
one insect. For each insect species, we transferred 50 llof each extract onto a cover slip, with individual sol-
vents or solely glass slides used as controls. After sol-
vents had dried, cover slips were placed under conidialshowers as described above for 2–3 h to achieve a den-
sity of >10 conidia/mm2, because previous studies
demonstrated that conidial density can affect germina-
tion (Hajek et al., 2002). Cover slips were then inverted
and incubated under humid conditions at 22� 1 �C for
22–24 h. Inversion of cover slips prevented any second-
ary conidia produced from landing on the cover slip.
Cover slips were then placed over drops of water onmicroscope slides. Conidial activity was recorded for 10
conidia in each of 10 fields of view at 400�, using phase
contrast on a compound microscope. Conidial activity
was scored as producing a germ tube or secondary co-
nidium or not germinating. Each type of solvent plus the
four controls was tested three times for each species
(three test solvents plus four controls� three replicates).
2.8. Data analysis
Conidial density and percent germination on L. dis-
par larvae were compared by cuticular region using
analysis of variance followed by post hoc comparisons
using the Bonferroni inequality to partition the overall aof 0.05. Data for conidial density and percent germi-
nation on cuculliines were not normally distributed. Tocompare conidial densities by intersegmental versus
segmental regions across cuculliine species, data were
transformed using logðxþ 1Þ and analyzed using a hi-
erarchical linear model with post hoc Tukey tests with
bioassay as a random effect. Comparisons of conid-ial densities on L. dispar larvae versus cuculliines by
cuticular region were made using non-parametric
Mann–Whitney tests. Percent conidial germination was
compared by region among L. dispar and cuculli-
ine species, or across regions for S. bicolorago, using
Mann–Whitney tests.
v2 tests were used to compare results from extract
studies. For each type of extract, germination andgrowth form were compared among species, with a
partitioned overall a of 0.05.
3. Results
Densities of conidia by body region varied dramati-
cally after inoculated larvae had been allowed to walk inexperimental cups for 12 h (Table 1). On L. dispar lar-
vae, E. maimaiga conidia were always more abundant
on the segmental cuticle and setae, with progressively
lower densities on the verrucae and the lowest densities
were found on intersegmental regions.
For four of the five cuculliine species tested, the dis-
tribution of conidia was reversed; the highest conidial
densities occurred in the intersegmental areas with sig-nificantly lower densities on the segmental cuticle (Table
1). The remaining cuculliine species, S. bicolorago, did
not follow this trend and conidial densities on inter-
segmental and segmental cuticle were the same. Cucul-
liines had no setae (S. signata and X. capax) or if setae
were present, they were relatively smaller than many of
the setae on L. dispar and were found in 6 37% of the
fields of view. Densities of conidia on setae of cuculliineswere extremely low (Table 1).
Lymantria dispar larvae always had more conidia on
setae than cuculliines (Table 1), at least partly because
they have many more setae. The hardened, raised ver-
Table 1
Mean densities (�SE) of E. maimaiga conidia by regions on the dorsal surfaces of lepidopteran larvae
Lepidopteran family Larval species No. of larvaeb Cuticular regiona
Intersegmental
(no./mm2)
Segmental
(no./mm2)
On setae
(no./mm2)
On verrucaed
(no./mm2)
Lymantriidae Lymantria dispar 44 0.9� 0.2 c 13.5� 0.7 a 11.7� 0.7 a 7:7� 0:4 b
Noctuidae, Cuculliinae Chaetaglaea sericea 9 12.5� 3.1 a* 2.6� 1.8 b* 0.3� 0.2* –
Eupsilia vinulenta 9 20.0� 2.7 a* 2.0� 0.3 b* 0.1� 0.0* –
Sericaglaea signata 9 12.2� 2.5 a* 1.0� 0.1 b* c –
Sunira bicolorago 9 11.5� 2.7 a* 8.8� 1.5 a 1.0� 0.4* –
Xylotype capax 8 17.8� 2.7 a* 2.8� 1.0 b* c –
a Letters following densities denote significant differences in conidial densities between cuticular regions for the species in that row (p < 0:05).
Asterisks following letters indicate that the conidial density for that region on that species differed from the density in the same region on L. dispar
larvae during the same bioassay (p < 0:05).b Total data for L. dispar are summarized in this table although only data from L. dispar assayed simultaneously with cuculliines were used for
separate tests.c Larvae of these species have no setae.dCuculliines do not have verrucae.
A.E. Hajek, C.C. Eastburn / Journal of Invertebrate Pathology 82 (2003) 12–22 15
rucae bearing setae on the segmental areas of L. disparalso had high conidial densities, but cuculliines do not
have these structures. Conidial densities on segmental
cuticle of L. dispar were greater than densities in this
region on cuculliines for four of the five species
(p < 0:05). Densities were equivalent comparing conidia
on segmental cuticle of L. dispar and S. bicolorago. The
relative densities were reversed between L. dispar and
the cuculliines for the intersegmental cuticle; for allcuculliines, intersegmental conidial densities were much
higher than for L. dispar.
None of the conidia germinated on the cuticles or
setae of E. vinulenta, S. signata, and X. capax (Table 2).
A few conidia germinated on S. bicolorago cuticle in
different regions and in the segmental region of C.
sericea (e.g., 2/369). For S. bicolorago, percent germi-
nation was greatest in the segmental region and on setae.However, due to the low numbers of conidia, this meant
that only 2 of the 38 conidia on setae germinated. On L.
dispar, where conidial densities were higher in the seg-
mental region and on the setae, highest percent germi-
nation occurred on the verrucae and in the segmental
region and germination on setae was lower. The lowest
germination was seen in the intersegmental region, as
with cuculliines. In fact, overall the percent of conidiathat germinated never approached 50%.
Scanning electron micrographs showed that cuculli-
ine cuticles were smooth, with a moist, mucous-like film
covering the entire cuticle. E. maimaiga conidia on
cuculliine cuticles were enveloped by this film (Fig. 1). L.
dispar cuticle appeared much more varied and did not
appear smooth, with many very small projections that
appeared to be covered by exudate. When drying cuc-ulliine cuticle for SEM, the film cracked in places (Fig.
1A), revealing underlying cuticle that was similar in
appearance to L. dispar cuticle (Fig. 2). On cuculliine
cuticles, conidia in intersegmental areas adhered to each
other, forming large aggregates and then many of the
conidia were not directly in contact with the cuticlesurface (Fig. 3). Conidia on the surface of L. dispar were
in direct contact with the cuticle, not covered by any
films over the host surface, and conidial aggregations
were not seen. On L. dispar, conidia on verrucae or in
segmental areas produced both short and long germ
tubes (Fig. 4). Conidia on setae that germinated were
often seen attached to germ tubes extending toward the
cuticle.The cuticle of L. dispar is much more hydrophobic
than cuculliine cuticle with contact angles ranging from
92.6� to 118.7� (Table 3). The difference in hydropho-
bicity among the species tested agreed with both the
attachment and germination results; conidia attached
and germinated on the more hydrophobic cuticle but
were dislodged and rarely germinated on the more hy-
drophilic cuticle.
3.1. Extract studies
Regardless of the extract used, P95% of the conidia
on cover slips with L. dispar extracts germinated (Table
4). Conidia on cover slips with hexane and chloroform
extracts from cuculliines also consistently germinated.
Fewer conidia exposed to methanol extracts from thefour cuculliine species germinated relative to conidia
exposed to methanol extracts from L. dispar (v2 tests;
p < 0:005).Greater than 90% of conidia on cover slips without
any extract or with solvents alone produced secondary
conidia. Most conidia that germinated on cover slips
with extracts from L. dispar developed germ tubes
(Table 4). Conidia exposed to hexane and chloroformextracts from cuculliines produced secondary conidia, as
did controls. Many of the germinating conidia exposed
to methanol extracts from cuculliines produced germ
tubes, although always fewer than conidia exposed to
L. dispar methanol extracts (v2 tests; p < 0:005).
Table 2
Percent germination (�SE) of E. maimaiga conidia on different regions of the dorsal surfaces of lepidopteran larvae
Lepidopteran family Larval species No. of larvaeb Cuticular regiona
Intersegmental (%) Segmental (%) On setae (%) On verrucaec (%)
Lymantriidae Lymantria dispar 44 2:3� 2:3 b 13.0� 1.4 a 12.1� 1.3 a 15:9� 1:6 a
Noctuidae, Cuculliinae Chaetaglaea sericea 9 0.0 0:7� 0:7* 0.0 —
Eupsilia vinulenta 9 0.0 0.0 0.0 —
Sericaglaea signata 9 0.0 0.0 d —
Sunira bicolorago 9 0:2� 0:2 b 5.5� 2.2 a* 2.2� 2.2 ab* —
Xylotype capax 8 0.0 0.0 d —
aLetters following densities denote significant differences among cuticular regions for that species (p < 0:05). Asterisks following letters indicate
that percent germination in that region for that species differed from percent germination in the same region on L. dispar larvae during the same
bioassay.b Total data for L. dispar are summarized in this table although only data from L. dispar assayed simultaneously with cuculliines were used for
separate tests.c Cuculliines do not have verrucae.d Larvae of these species have no setae.
16 A.E. Hajek, C.C. Eastburn / Journal of Invertebrate Pathology 82 (2003) 12–22
4. Discussion
We conducted conidial showers so that both host and
non-host larvae would receive the same concentrations
of conidia over their entire bodies. However, we did not
find equivalent densities on the bodies of hosts (L. dis-par) and non-hosts (cuculliines) 12 h later. For the five
cuculliine species, we consistently found the majority of
Fig. 1. Dorsal cuticle of X. capax larva with conidia of E. maimaiga. (A) Film covering a conidium plus underlying cuticle seen through cracks in the
film caused during processing for SEM. Bar, 20lm. (B) Group of film-covered conidia on cuticle. Bar, 50 lm.
A.E. Hajek, C.C. Eastburn / Journal of Invertebrate Pathology 82 (2003) 12–22 17
conidia in aggregations in intersegmental membranes.
Likewise, conidia of hyphomycetes have been found in
aggregations in intersegmental folds in beetle larvae
(Fernandez et al., 2001; Vey et al., 1982), grasshoppers
(Inglis et al., 1995) and thrips (Schreiter et al., 1994). Incontrast, Wraight et al. (1990) found no difference in
densities of conidia of the entomophthoralean Z. radi-
cans across regions of leafhopper bodies. SEM showed
that E. maimaiga conidia in the intersegmental areas on
cuculliines were enveloped by a film that covered the
cuculliine cuticle and conidia were found in large ag-
gregations in intersegmental areas adhering to each
other. We hypothesize that the accordion-like move-ment when larvae walked moved the poorly attached
conidia to the intersegmental areas where they became
aggregated. Conidia of other entomopathogens are
known to be moved after initial deposition on cuticles
but generally they are reported as being lost. Conidia of
Paecilomyces fumosoroseus were dislodged from ventral
surfaces when larvae of the diamondback moth, Plutella
xylostella walked (Altre et al., 1999). Many conidia ofVerticillium lecanii were dislodged from dorsal surfaces
after 24 h on an ant, a springtail and two carabid species,
but fewer conidia were dislodged from aphids, the typ-
ical hosts (Sitch and Jackson, 1997). A high percentage
of conidia of Conidiobolus obscurus were lost from the
cuticles of host aphids within 2 h of application (Latg�eeet al., 1982). In the extreme, conidia of the entomoph-
thoralean Z. radicans did not adhere when applied tonon-host leafhoppers (McGuire, 1985).
In contrast to the locations of conidia on the cuculli-
ines, conidia on L. dispar larvae were found individually,
often on segmental areas, setae and verrucae and these
conidia did not appear to have been moved during larval
walking. In agreement, studies with entomopathogenicHyphomycetes also found higher conidial densities in
areas of the cuticle with spines (Boucias et al., 1988) or
setae (Pekrul and Grula, 1979; Sosa-Gomez et al., 1997).
It has been suggested that conidia are trapped in these
areas, although with L. dispar it also seems likely that
areas with setae do not move as much to dislodge conidia
when larvae walk. On L. dispar, conidia were also fre-
quently found on the abundant setae but this did notprevent conidia from germinating and growing as germ
tubes toward the cuticle. Based on previous observations,
we believe that the low number of conidia in interseg-
mental regions is possibly due to rupture of these well-
attached conidia when larvae walked and intersegmental
regions folded inwards (Hajek et al., 2002). Better adhe-
sion of conidia to L. dispar cuticle that is more hydro-
phobic than cuculliine cuticle agrees with findings ofincreased adhesion of plant pathogenic fungi associated
with higher surface hydrophobicity (Kuo and Hoch,
1996;Terhune andHoch, 1993).Our results are consistent
with results from previous studies finding only low per-
centages of entomophthoralean conidia that germinate
produce germ tubes for subsequent penetration (Brey
et al., 1986; Nadeau et al., 1996; Wraight et al., 1990);
evenunder ideal circumstances, themajority of conidia onL. dispar larval cuticle did not germinate.
Fig. 2. Dorsal cuticle of L. dispar larva with conidium of E. maimaiga. Bar, 20 lm.
18 A.E. Hajek, C.C. Eastburn / Journal of Invertebrate Pathology 82 (2003) 12–22
We hypothesize that the mucous film on the cuculli-
ines acts as an external protection for these larvae thathave virtually no setation and live part of their lives at
the soil surface. This film acts as a physical barrier,
preventing adhesion of conidia to the underlying larval
cuticle and it deserves further study. The film-engulfedconidia on cuculliines rarely germinated. These results
would agree with suggestions that germination is greater
Fig. 3. Large aggregations of E. maimaiga conidia on the dorsal cuticle of cuculliine noctuids. (A) X. capax. Bar, 230lm. (B) S. bicolorago. Bar,
165lm. For both species, the film covering the larval surface became dry and cracked when processed for SEM.
A.E. Hajek, C.C. Eastburn / Journal of Invertebrate Pathology 82 (2003) 12–22 19
with increased cuticular-conidial contact (St. Leger et al.,
1991). In contrast, the many setae of L. dispar that arethought to have evolved for protection seem also to
increase the surface area for attachment of E. maimaiga
conidia; to further evaluate whether setae protect
against or increase chance of infection, the numbers ofconidia on setae that actually are responsible for infec-
tions should be evaluated.
Fig. 4. Germination of E. maimaiga on L. dispar cuticle. (A) Penetration close to conidium. Bar, 20lm. (B) Growth of long germ tubes across the
cuticle surface. g, germ tube; c, conidium. Bar, 85lm.
20 A.E. Hajek, C.C. Eastburn / Journal of Invertebrate Pathology 82 (2003) 12–22
Methanol extracts of the cuticle of cuculliine species
reduced germination, suggesting that a methanol-solu-
ble component of the cuculliine cuticle may be fungi-
static or fungitoxic. Compounds present on cuticles of
some insects are known to inhibit attachment, germi-
nation and appressorium formation, steps that are pre-
cursors to cuticular penetration (St. Leger, 1991). In this
study, all extracts from L. dispar induced germ tubeformation. Curiously, conidia exposed to cuculliine
methanol extracts that were able to germinate produced
germ tubes rather than secondary conidia, suggesting a
possible stimulatory effect. Studies with the entomoph-
thoralean Erynia variabilis demonstrated that exposure
to chloroform/methanol extracts of host fly cuticle
produced germ tubes and not secondary conidia (Ker-
win, 1984). Exposure of C. obscurus conidia to chloro-form/methanol extracts from hosts or non-hosts also
induced germ tube production (Boucias and Latg�ee,1988); these authors suggested that this stimulatory re-
sponse is probably relatively nonspecific. Our findings
suggest that there is some component in methanol ex-
tracts from cuculliine cuticle that induces germ tube
formation but some other chemical components are
present that inhibit germination.In the field one of the few species that has been col-
lected infected by E. maimaiga was one individual of S.
bicolorago, suggesting that sometimes this pathogen in-
fects this species in nature (Hajek et al., 2000). Whether
that infection was initiated by penetration directly
through the cuticle or through a wound is not known.Results from this study agree with field collections be-
cause this is the one cuculliine species studied that had
the highest chance of becoming infected based on bio-
assay results.
Knowledge of host specificity is necessary for identi-
fying effective control agents but also for reducing non-
target effects. Effects of biological control agents on
non-target organisms are presently under close scrutiny(Follett and Duan, 2000; Wajnberg et al., 2001). Al-
though not always available, effective agents with nar-
row host specificity are desired for classical biological
control. Because we cannot test all organisms that are
present in the environment, the ability to predict whe-
ther non-target species might be affected is critically
important. One of our goals in undertaking this study
was to investigate whether species within the samesubfamily had similar determinants of host specificity;
can we use host taxonomy to help predict susceptibility?
Studies with Entomophthorales have shown that infec-
tion can occur in different families within an insect order
but there is a trend for greater levels of infection in
specific groups. For E. muscae isolated from a calli-
phorid fly but maintained in the laboratory on Musci-
dae, the greatest infection was in one species of muscidtested (Steinkraus and Kramer, 1987). For Z. radicans
isolated from cicadellid leafhoppers, the greatest infec-
tion was seen in cicadellids, although only in 3 of the 4
species tested (McGuire et al., 1987). For E. maimaiga
the greatest infection was consistently found only for
species in the same host family from which the fungus
had been isolated, the Lymantriidae (Hajek et al., 1995).
In this study, we found that species within the noctuidsubfamily Cuculliinae consistently displayed similar at-
tributes that reduced risk of infection by E. maimaiga;
these results would suggest that perhaps lower level
taxonomic relationships, i.e., subfamily in this case,
could help in predicting patterns of host specificity.
However, further studies with other systems should be
conducted before relying on phylogenetic relatedness to
determine safety.
Table 3
Average contact angles for cuticles of lepidopteran larvae
Lepidopteran
family
Species Contact angle
(mean� SE)
Lymantriidae Lymantria dispar 170.8� 6.9
Noctuidae,
Cuculliinae
Chaetaglaea sericea 92.6� 3.0
Eupsilia vinulenta 118.7� 0.7
Sericaglaea signata 95.1� 5.1
Sunira bicolorago 111.6� 12.1
Xylotype capax 112.7� 2.4
Table 4
Percent germination and production of germ tubes (�SE) by E. maimaiga on extracts of lepidopteran larval cuticlesa
Species Germinationb (%) Germ tubesb ;c
Methanol Chloroform Hexane Methanol Chloroform Hexane
Lymantria dispar 96:0� 1:1 a 95:0� 2:9 a 96:0� 1:0 a 98:6� 1:4 a 72.8� 21.6 a 82.8� 12.8 a
Eupsilia vinulenta 50:0� 5:9 c 97:7� 0:3 a 92:5� 0:4 a 60:3� 13:4 d 0.7� 0.7 d 0.5� 0.4 d
Sericaglaea signata 62:5� 3:8 b 94:3� 1:2 a 94:3� 1:3 a 91:2� 1:9 bc 4.6� 0.7 c 16.9� 3.1 b
Sunira bicolorago 61:0� 5:4 bc 98:0� 0:6 a 97:0� 1:5 a 91:8� 5:6 b 29.2� 14.3 b 19.8� 6.3 b
Xylotype capax 59:0� 1:5 bc 94:7� 1:5 a 95:5� 2:0 a 83:8� 9:7 c 3.9� 2.3 cd 6.8� 1.1 c
aCover slips with individual extracts or no extract were used for controls and >90% of conidia on control cover slips always germinated and
produced secondary conidia.bDifferent letters within a column demonstrate significant differences between percentages (v2 tests each tested at a ¼ 0:005).c Percent production of germ tubes versus secondary conidia.
A.E. Hajek, C.C. Eastburn / Journal of Invertebrate Pathology 82 (2003) 12–22 21
Acknowledgments
We thank C. Daugherty for her excellent eye, deft
touch, and patience with the scanning electron micro-
scope. Thanks to D. Schweitzer and T. Hupf for col-
lection and initial rearing of cuculliines. A. Savage
helped rear larger cuculliines and M. Bertoia, K. Poole,
K.-L. Tsai, and K. Zuniga helped rear L. dispar larvae
and infect larvae. J.L. Kerwin and J.A.A. Renwickhelped with suggestions for procedures during cuticular
chemistry studies and J.L. Kerwin provided helpful
comments on the manuscript. F.M. Vermeylen assisted
with the use of hierarchical linear models. Y. Ando,
S.-H. Kang, and X. Li helped with use of the goniometer
belonging to the Cornell University, Department of
Materials Science and Engineering. This study was
funded by USDA, NRICGP #96-04343.
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