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Transovarial transmission of Rickettsia and organ-specific infection of the whitefly Bemisia 1
tabaci 2
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Marina Brumin1, Maggie Levy2 and Murad Ghanim1# 4
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1Department of Entomology, the Volcani Center, Bet Dagan 50250, Israel and 2 Department of 6
Plant Pathology and Microbiology, Robert H. Smith Faculty of Agriculture, Hebrew University 7
of Jerusalem, Rehovot 76100, Israel. 8
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#Correspondence: M. Ghanim, E-mail: [email protected] 11
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Running title: Rickettsia – Whitefly interactions 14
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Copyright © 2012, American Society for Microbiology. All Rights Reserved.Appl. Environ. Microbiol. doi:10.1128/AEM.01184-12 AEM Accepts, published online ahead of print on 1 June 2012
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The whitefly Bemisia tabaci is a cosmopolitan insect pest that harbors Portiera 24
aleyrodidarum, the primary obligatory symbiotic bacterium, and several facultative 25
secondary symbionts. Secondary symbionts in B. tabaci are generally associated with the 26
bacteriome, ensuring their vertical transmission; however, Rickettsia is an exception and 27
occupies most of the body cavity, except the bacteriome. The mode of Rickettsia transfer 28
between generations and its subcellular localization in insect organs were not investigated. 29
Using electron and fluorescence microscopy, we show that Rickettsia infects the digestive, 30
salivary and reproductive organs of the insect, however, it was not observed in the 31
bacteriome. Rickettsia invades the oocytes during early developmental stages and resides in 32
follicular cells and cytoplasm; it is mostly excluded when the egg matures, however, some 33
bacterial cells remain in the egg, ensuring their transfer to subsequent generations. 34
Rickettsia was localized to testicles and the spermatheca, suggesting a horizontal transfer 35
between males and females during mating. The bacterium was further observed at high 36
amounts in midgut cells, concentrating in vacuolar-like structures, and was located in the 37
hemolymph, specifically at exceptionally high amounts around bacteriocytes and in fat 38
bodies. Further infected organs by Rickettsia included the primary salivary glands and 39
stylets, sites of possible secretion of the bacterium outside the whitefly body. The close 40
association between Rickettsia and B. tabaci digestive system might be important for 41
digestive purposes. The vertical transmission of Rickettsia to subsequent generations occurs 42
via the oocyte and not, like other secondary symbionts, the bacteriome. 43
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INTRODUCTION 48
The intimate interactions between endosymbionts and their arthropod hosts are well established 49
for obligate primary symbionts such as Buchnera in aphids and Carsonella in psyllids (3, 27). 50
These bacteria are housed within specialized cells termed bacteriocytes and aggregate together to 51
form an organ termed bacteriome (3, 12, 56). Primary endosymbionts provide the host with 52
essential amino acids to complete their diet, and are therefore necessary for host survival and 53
development (12). In contrast, secondary symbionts are not essential and until recently, their 54
effect on their host's biology was underestimated. In the past few years however, their relevance 55
has become a matter of interest and accumulating data suggest that they can play a significant 56
role in the biology of their hosts (56). To date, secondary symbionts have been reported to be 57
involved in reproductive manipulations, host plant utilization, and ability to cope with 58
environmental factors such as response to heat stress and chemical insecticides (8, 11, 43, 46, 49, 59
57, 58). The reported localization patterns of secondary symbionts are diverse and vary within 60
the host body. The bacteria can be either diffusely distributed throughout the entire host body or 61
restricted to specific tissues. For example, secondary symbionts have been reported from the 62
hemolymph of many insect taxa (15, 28, 34, 67), primary bacteriocytes in whiteflies (39, 63), 63
secondary bacteriocytes and sheath cells mainly in aphids (34, 55, 61, 67), salivary glands (54, 64
59, 60), Malpighian tubules (13) and reproductive organs (28, 32, 41, 60, 68). 65
Like other phloem-feeders, the sweetpotato whitefly, Bemisia tabaci (Gennadius) 66
(Hemiptera: Aleyrodidae), harbors a diverse array of endosymbionts, including the primary 67
endosymbiont Portiera aleyrodidarum (3), and several other facultative secondary symbionts, 68
including Rickettsia, Hamiltonella, Wolbachia, Arsenophonus, Cardinium, and Fritschea (3, 38). 69
B. tabaci is a complex of several cryptic species, also termed biotypes, which differ genetically 70
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and biologically. The most widespread and damaging biotypes are B and Q [recently termed 71
Middle East Asia Minor 1 (MEAM1) and Mediterranean (MED), respectively] (24). The B 72
biotype from Israel has been associated with Hamitonella, while the Q biotype is associated with 73
Wolbachia and Arsenophonus. Both biotypes harbor Rickettsia with infection rates ranging from 74
22 to 100% (17). Neither biotype harbors Cardinium or Fritschea (17). A molecular 75
phylogenetic analysis based on 16S rDNA and gltA sequences revealed that Rickettsia sp. from 76
B. tabaci belongs to the group consisting of Rickettsia bellii from ticks and Rickettsia spp. from 77
herbivorous arthropods such as aphid and leafhopper. This Rickettsia shares 99 and 97% 78
similarity with R. bellii 16S rDNA and gltA sequences, respectively (38). Rickettsia symbionts 79
have been further identified from a wide variety of invertebrates such as aphids (15), leafhoppers 80
(22), lady bird beetles (69), bruchid beetles (33), leeches (47) and ticks (6). 81
All secondary symbionts in B. tabaci co-localize with the primary symbiont inside the 82
bacteriocytes, ensuring their vertical transmission. However, only Rickettsia localizes outside the 83
bacteriocytes and appears in most of the body cavity except the bacteriocytes (39). In only one 84
case, Rickettsia was described co-localizing with the primary symbiont inside the bacteriocyte 85
(14, 39). It is still unclear how Rickettsia that localizes outside the bacteriosome is transferred 86
and spread in B. tabaci populations, especially that it can reach high prevalence and near fixation 87
in natural populations as was recently shown in Arizona (45). The later study has further shown 88
that Rickettsia-infected B. tabaci females exhibit high fitness benefits such as increased 89
fecundity, a greater rate of survival, and host reproduction manipulation via the production of a 90
higher proportion of daughters (45). Additional studies have shown that the presence of 91
Rickettsia in B. tabaci populations influenced the whitefly’s response to heat stress by benefitting 92
its host under high temperatures (11), and has also shown to increase the whitefly's susceptibility 93
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to chemical insecticides (49). Studies on Rickettsia from other invertebrates have revealed 94
diverse effects of the bacteria on their hosts. For example, in the pea aphid Acyrthosiphon pisum, 95
Rickettsia-infected individuals showed lower fresh body weight, reduced fecundity and 96
significantly suppressed densities of Buchnera, suggesting a negative effect of Rickettsia (16, 97
61). Reproductive manipulation and Rickettsia-associated parthenogenesis have been shown in 98
the endoparasitoid Neochrysocharis formosa (42), and in the parasitoid wasp Pnigalio soemius 99
(37), as has Rickettsia-associated male-killing in beetles (71, 69), and involvement in oogenesis 100
of booklice (72). 101
To unravel additional biological functions for Rickettsia in B. tabaci, including possible 102
transmission routes, the spatial subcellular localization of the bacterium in internal organs and 103
cells must be determined. Little is known about the specific subcellular localization of Rickettsia 104
within arthropod hosts. To hypothesize possible biological functions and interactions with the 105
insect host, fluorescence and electron microscopy were used here to show that Rickettsia 106
occupies specific, previously undescribed niches and organs within B. tabaci’s digestive, salivary 107
and reproductive organs and cells. The presence of the bacterium in these organs gives some clue 108
as to the specific undescribed interactions and possible transmission routes, suggests possible 109
horizontal transfer of the bacterium during mating, and confirms a recent report suggesting that 110
horizontal transmission of Rickettsia might be plant-mediated (14). 111
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MATERIALS AND METHODS 113
Insects and rearing conditions. Rickettsia-free and Rickettsia-containing B-biotype B. tabaci 114
populations were reared on cotton seedlings (Gossypium hirsutum L. cv. Acala) maintained 115
inside insect-proof cages and growth rooms under standard conditions of 25 ± 2 ºC, 60% relative 116
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humidity and a 14 h light/10 h dark photoperiod. Identification of the B biotype was based on 117
microsatellite markers (23). The two strains of B. tabaci biotype B used in this study were 118
established by selection of isofemale strain as previously described (11). The original B biotype 119
population used to establish the isofemale strains was collected from Ayalon valley in Israel 120
(31° 52′ 3″ N, 34° 57′ 34″ E) in 1996 and cultured under laboratory conditions. This population 121
tested positive for Portiera and Hamiltonella. 122
DNA extraction and PCR amplification. To confirm the presence of Rickettsia in each adult B. 123
tabaci individual, 20 whiteflies were individually homogenized in lysis buffer as previously 124
described (31.). The lysate was then incubated at 65 ºC for 15 min followed by incubation at 95 125
ºC for 10 min. The samples were tested for the presence of Rickettsia by PCR using Rickettsia-126
specific primers for amplification of the 16S rDNA gene fragment: Rb-F 5’-127
GCTCAGAACGAACGCTATC-3’ and Rb-R 5’-GAAGGAAAGCATCTCT GC-3’ (38). The 128
reaction was carried out in a 20-µl volume containing 2 µl template DNA lysate, 20 pmol of each 129
primer, 10 mM dNTPs, 1X DreamTaq buffer and 1 U DreamTaq DNA Polymerase (Fermentas). 130
PCR-amplified products were visualized on a 1% agarose gel containing ethidium bromide. To 131
detect Rickettsia in specific organs using PCR, B. tabaci midguts, stylets, primary salivary 132
glands and hemolymph were dissected under binocular in 1X phosphate buffered saline (PBS), 133
washed and subjected to the above-described lysis-PCR amplification. The reaction contained 10 134
µl of template DNA lysate. 135
FISH. FISH was performed as previously described (38). Briefly, specimens were fixed 136
overnight in Carnoy’s fixative (chloroform:ethanol:glacial acetic acid, 6:3:1, v/v), then 137
decolorized in 6% H2O2 in ethanol for 2 h and hybridized overnight in hybridization buffer (20 138
mM Tris-HCl pH 8.0, 0.9 M NaCl, 0.01% w/v sodium dodecyl sulfate, 30% v/v formamide) 139
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containing 10 pmol fluorescent probes per ml. Dissected midguts, salivary glands and ovaries 140
were fixed for 5 min in Carnoy’s fixative and hybridized overnight. For specific targeting of 141
Portiera and Rickettsia, BTP1-Cy3 (5’-Cy3-TGTCAGTGTCAGCCCAGAAG-3’) and Rb1-Cy5 142
(5’-Cy5-TCCACGTCG CCGTCTTGC-3’) probes were used, respectively. Nuclei were stained 143
with 4’,6’-diamidino-2-phenylindole (DAPI) (0.1 mg ml-1). The stained samples were mounted 144
whole in hybridization buffer and viewed under an IX81 Olympus FluoView500 confocal 145
microscope. For each stage, at least 15 specimens were viewed under the microscope to confirm 146
reproducibility. Optical sections (0.7-1.0 μm thick) were prepared from each specimen. 147
Specificity of detection was confirmed using no-probe and Rickettsia-free whitefly controls. 148
Electron microscopy. Detached adult whitefly abdomens and heads were fixed overnight in 149
2.5% glutaraldehyde in 1X PBS at 4 ºC and processed using a standard method for TEM: rinsing 150
in 1X PBS buffer, osmification, another rinse in 1X PBS buffer, dehydration in an ascending 151
ethanol series, acetone incubation and embedding in epoxy resin Agar 100 (Agar Scientific, 152
Essex, England). Thin sections (60–90 nm) were cut using an ultramicrotome, stained with 153
aqueous uranyl acetate and lead citrate and examined in a Tecnai 12 electron microscope 154
(Philips/FEI, Eindhoven, The Netherlands). 155
156
RESULTS 157
General distribution of Rickettsia in the adult hemolymph. The distribution of Rickettsia was 158
monitored in whole insects and dissected organs by means of FISH and TEM. The bacterium 159
was generally distributed throughout the body cavity, appearing in the head, thorax and abdomen 160
(Fig. 1A). In some cases, the bacterium was heavily concentrated around bacteriocytes, and was 161
less observable in other locations (Figs. 1B–F). The latter phenotype was not significantly 162
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correlated with whitefly sex or age. Many serial confocal and TEM sections indicated that 163
Rickettsia is not present in bacteriocytes in the adult female stage, even when the bacterium cells 164
are highly abundant around bacteriocytes. In only one case Rickettsia-like cells were observed 165
attached to the outer surface of the bacteriocyte, and potentially internalized by the bacteriocyte 166
(Fig. 1F). These observations suggest that the mode of vertical transmission to the next 167
generation via bacteriocytes cannot explain the high abundance and perfect vertical transmission 168
of Rickettsia from the female to its offspring. 169
170 Oocyte-mediated vertical transmission of Rickettsia. We tested the hypothesis that Rickettsia 171
hitchhikes with the bacteriocyte for vertical transmission via the oocyte, as was previously 172
described for the other endosymbionts in whiteflies (12, 20, 39, 40, 65). The results indicated 173
that Rickettsia is the exception. The possibility for vertical transmission via free bacteriocytes 174
was excluded based on TEM and confocal serial sections (Fig. 1). Rickettsia was not seen 175
penetrating bacteriocytes that were already contained in the oocyte or free in the hemolymph, 176
suggesting that this is not a route of oocyte entry. The path of Rickettsia entrance into developing 177
oocytes was followed, focusing on different developmental stages of the oocyte. Indeed, 178
Rickettsia invaded the oocytes in the very early stages of development, and high levels of 179
bacterial cells were concentrated inside the oocytes at all developmental stages, especially the 180
younger stages 1 and 2 (Figs. 2A and C-F). The concentration of bacterial cells decreased in the 181
more mature oocytes, especially in their central part (Figs. 2A–E), while they were not observed 182
in free bacteriocyte cells surrounding the developing oocytes (Fig. 2F). The location of Rickettsia 183
in the developing oocytes was further explored using serial TEM sections. Young oocytes in 184
stages 1 to 3 contained larger amounts of Rickettsia cells in the cytoplasm and in the surrounding 185
follicular cells (Figs. 3A–C). However, oocytes in later stages 4 and 5 of development contained 186
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bacterial cells mostly in the surrounding follicular cells and less Rickettsia inside the oocyte 187
cytoplasm (Figs. 3D and E). At stage 5 of development, the oocyte is almost completely filled 188
with fat vacuoles and droplets and bacterial cells were not observed in the cytoplasm (Fig. 3E). 189
190 Organ- and tissue-specific infection. The general distribution of Rickettsia in B. tabaci as 191
observed by FISH led us to monitor its presence in other whitefly organs and subcellularly, using 192
both TEM and FISH analyses. The organs and tissues analyzed were the digestive and salivary 193
systems including the midgut, salivary glands and stylet. Furthermore, the male and female 194
reproductive organs were analyzed for infection by Rickettsia, and the possible sexual transfer of 195
the bacterium between infected and healthy individuals was tested. Other tissues that were tested 196
for infection were flight muscles in the thorax and fat bodies in the abdomen. 197
Experiments employing dissected midguts and Rickettsia-specific probe showed that the 198
midgut contains very high amounts of bacterial cells, unlike many of the other organs in B. 199
tabaci (Fig. 4). Rickettsia cells sometimes clustered in groups inside vacuolar-like structures 200
(Fig. 4A and Figs. 5C and D), and were easily distinguished by TEM and FISH (Fig. 4A and C 201
and Figs. 5A and B). The bacterium cells were never observed in the midgut lumen (Figs. 4B and 202
C and Figs. 5A and C). Midguts dissected from younger 1-2 days old males and females, as well 203
as older 7-14 days individuals contained similar localization patterns of Rickettsia. 204
FISH analysis detected Rickettsia in the primary salivary glands (Fig. 6B), and this result 205
was confirmed using TEM (Figs. 6C and D). The bacterial cells were located in cells 1 and 2 206
described by Ghanim et al. (36). These cells contain exceptionally large nuclei, electron-dense 207
granules and lipid-like accumulations, but their cytoplasm is less dense than that of the other 208
cells in the gland (36), and were hypothesized to act in producing the gelling saliva required for 209
the stylet penetration in the plant leaf. Using FISH, we were able to confirm the presence of 210
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Rickettsia in the whitefly stylet, along the interlocked maxillae through which the food and 211
salivary canals pass (Fig. 7). Interestingly, FISH signal was also observed on the mandibles that 212
surround these two canals (Fig. 7). At this resolution, we were not able to determine whether the 213
signal exists only in the food, salivary, or both canals. 214
The reproductive organs of both B. tabaci males and females were monitored for the 215
presence of Rickettsia. The bacterium was detected by FISH in dissected testes from B. tabaci 216
males (Figs. 8A–D) and dissected spermathecae from fertilized females (Figs. 8E and F). 217
Interestingly, the labeling was observed in all stages of spermatogenesis in the primary cells of 218
the primary glands in the testes and spermathecae; however, less Rickettsia cells were associated 219
with the mature spermatids (Fig. 8D). This observation suggested that Rickettsia might be 220
sexually transmitted between individuals, one mechanism for horizontal transfer, thus affording a 221
potential route for Rickettsia maintenance in B. tabaci populations. Indeed, copulation 222
experiments that we conducted on artificial diet between 30 Rickettsia-infected females with 30 223
uninfected males and vice versa, showed that Rickettsia could be detected by PCR in some of the 224
uninfected counterparts (data not shown). 225
Further tissues in which Rickettsia cells were detected are muscle band cells in the flight 226
muscles located in the thorax of adult males and females using TEM ultrathin sections (Fig. 9A), 227
and fat bodies in the hemolymph of both sexes (Figs. 9B and C ). 228
229
DISCUSSION 230
In the present study we obtained new data regarding the infection of B. tabaci by Rickettsia. We 231
further showed organ-specific distribution and possible relevance to the high abundance of 232
Rickettsia in the insect populations (45). The high abundance of Rickettsia in the hemolymph, 233
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especially around bacteriocytes, first suggested possible vertical transmission via the oocyte by 234
hitchhiking with bacteriocyte as was previously suggested (38). Although it is widely accepted 235
that many bacterial endosymbionts are vertically transmitted into newly developed oocytes with 236
bacteriocytes, especially in whiteflies (12, 20, 38, 39, 40, 65), the results presented here refute 237
this hypothesis and show that Rickettsia is the exception (Fig. 1). TEM serial sections did not 238
detect Rickettsia cells inside bacteriocytes, and only the abundant primary symbiont Portiera and 239
the secondary symbiont Hamiltonella, were always associated with bacteriocytes (Figs. 2 and 3). 240
TEM sections through the developing oocytes and bacteriocytes showed that younger oocytes are 241
heavily infected with Rickettsia cells, which are mostly excluded and concentrate in follicular 242
cells, with development. It is thus likely that Rickettsia cells are transferred to the next 243
generation via the egg by residing in the follicular cells. The observation of younger oocytes 244
being filled with bacterial cells corresponds with the fact that young oocytes are more permeable 245
to materials in the hemolymph than developed ones, which exhibit more selective barriers. 246
Follicular cells facilitate the uptake of various materials from the hemolymph to the oocyte and 247
are involved in the synthesis and transport of precursors of both the internal vitelline and external 248
chorion envelopes that surround the oocyte (53). Rickettsia has been shown to invade the 249
follicular cells of parasitic wasps of B. tabaci (18), but bacterial cells were not observed beyond 250
the follicular cells. Other bacterial symbionts such as Wolbachia in Drosophila melanogaster 251
(32), and Cardinium in the leafhopper Scaphoideus titanus (60), have been shown to invade the 252
reproductive system, including follicular cells, ensuring their own transmission to the next 253
generation. Our observation of Rickettsia invading the follicular cells and the cytoplasm of 254
developing oocytes suggests that this bacterium uses the oocyte, not the bacteriocyte route, to 255
ensure its transmission to the next generation. 256
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For the first time, we show that B. tabaci midgut is heavily infected with Rickettsia. It is 257
unclear how or when Rickettsia enters and becomes established in the midgut cells. One 258
possibility is the oocyte and egg cells that give rise to intestinal tissue in later developmental 259
stages. The high concentration of Rickettsia in the midgut and its specific localization in the 260
vacuoles (Figs. 5B and D), suggest a possible role in food digestion. Midgut-associated 261
symbionts have been reported from many arthropods, such as the Mediterranean fruit fly, tsetse 262
fly, silkworms, termites and stinkbugs, among many others (46). The diversity of midgut 263
microbes is enormous: they belong to various genera and exhibit different localization patterns, 264
modes of transmission and functional roles, depending on both the bacteria and the host (25, 29). 265
Intestinal microbes may contribute to food digestion, provide essential amino acids and vitamins 266
to the host, fix nitrogen and keep out potentially harmful microbes (2, 4, 5, 10, 66, 35). Gut 267
microorganisms also possess metabolic properties that are absent in insects, thus enabling the 268
phytophagous insects to overcome biochemical barriers to herbivory by detoxifying plant 269
allelochemicals such as flavonoids, tannins, and alkaloids (7, 25, 26). However, the gut bacteria 270
explored to date are phylogeneticlly distant from the α-proteobacterial group of Rickettsia and 271
nothing is known about the latter's functional role in the digestive system. 272
Interestingly, Rickettsia cells were found in the primary salivary glands (Fig. 6). 273
Occurrence of bacteria in the salivary glands has been reported from different insect species, and 274
has been suggested to serve as a route for its horizontal transmission to plants or other 275
intermediate hosts (28, 54, 59, 60). The first and strongest evidence of horizontal transmission of 276
symbiotic bacteria via an insect's plant host was reported for the leafhopper Euscelidius 277
variegates (59) and the pathogenic symbiont BEV. Similar to other sap-sucking arthropods, the 278
horizontal transmission of B. tabaci symbionts requires the passage of the bacterial cells through 279
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several barriers, most importantly from salivary gland cells through the salivary duct to the 280
stylet. Our results show that presence of Rickettsia in the whitefly stylet is restricted to the 281
interlocked maxillae through which the food and salivary canals pass (Fig. 7). Interestingly, 282
FISH signal was also observed on the mandibles that surround these two canals (Figure 7). At 283
this resolution, we were not able to determine whether the signal exists in the food, salivary, or 284
both canals; however, the presence of the bacterium in either one of these canals suggests its 285
passage into or out of the whitefly body with plant sap. It has been recently suggested that 286
Rickettsia is horizontally transmitted through the plant host (14), where it was observed in the 287
plant sieve elements following feeding of Rickettsia-infected whiteflies and was also acquired 288
from the plant by Rickettsia-free whiteflies. Combining our microscopy findings with the recent 289
report of Caspi-Fluger et al. (14) provides stronger evidence for the horizontal transfer of 290
Rickettsia in B. tabaci through the plant host. 291
Our results indicated the infection of male and female reproductive tissues by Rickettsia, 292
and preliminary copulation experiments that we performed, using artificial diet, suggest possible 293
transfer of Rickettsia during mating (Fig. 8 and unpublished data). These results, in addition with 294
the recent study suggesting horizontal transmission through the plant (14), might explain the 295
exceptionally high prevalence of Rickettsia in natural populations, such as its establishment and 296
near fixation in populations of B. tabaci in Arizona in just 6 years (45). In the later study, 297
Rickettsia-infected whiteflies produced more offspring, had higher survival rates, developed 298
faster and produced a higher proportion of daughters. The observed sex ratio bias might be 299
attributed in part to possible effects of Rickettsia on the Rickettsia-infected sperm in the female 300
spermatheca, which is used by the female to fertilize eggs. In this arrhenotokous mode of 301
reproduction, fertilized eggs develop to females while unfertilized eggs develop to males. 302
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Wolbachia is the most studied microorganism with respect to associations with insect 303
reproductive organs, which induce cytoplasmic incompatibility (CI) and reproductive 304
manipulations in several insect species, and was associated with breakdown of spermatogenesis 305
(30). Several other bacterial symbionts, which reside in male and female reproductive organs and 306
induce reproductive manipulations, were further described, including Cardinium (21, 73, 74), 307
Candidatus Blochmannia floridanus (62) and Arsenophonus (70). A spotted fever group 308
Rickettsia was previously described in the spermatogonia, spermatocytes and maturing 309
spermatids of its male tick vector Ixodes ricinus, and it could be sexually transmitted to females, 310
but it did not have negative effects on the developing eggs (44). 311
The presence of Rickettsia in muscle cells was somewhat surprising, and it is unclear 312
whether this has any effect on the muscle-related biology of the whitefly, such as flight. Several 313
bacterial symbionts that have been previously localized to thoracic and muscle tissues, of their 314
hosts were associated with inducing negative and even pathogenic effects on the host. The best 315
studied examples of Rickettsia species that infect muscle tissues stem from pathogenic Rickettsia 316
species and their interactions with their arthropod vectors. Few examples include the two major 317
groups of pathogenic Rickettsia: the spotted fever and typhus groups, and their interactions with 318
their tick vectors (64), and Anaplasma marginales (Rickettsiales: Anaplasmataceae) in the male 319
Rocky Mountain wood tick Dermacentor andersoni (48). 320
The association of Rickettsia with B. tabaci fat bodies was not expected as the presence 321
and functional association of endosymbionts in fat bodies is not common in insects. Only 322
endosymbionts from the Blattabacteria that co-evolved with termites and cockroaches were 323
reported from the fat body, but no specific functional role for these endosymbionts has been 324
assigned (19, 50, 52). In whiteflies, vitellogenin and possibly other important proteins are 325
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produced in the fat body, and thus the presence of Rickettsia might indicate a role in these 326
processes. 327
In conclusion, FISH and TEM analyses showed the presence of Rickettsia endosymbiont 328
in B. tabaci whiteflies. Rickettsia was localized to major organs involved in the host's 329
reproductive, feeding, circulation and secretion systems. Interestingly, the broad spectrum of 330
Rickettsia-infected tissues in B. tabaci documented in this study resembles that found for the 331
pathogenic Rickettsia felis in cat fleas (1, 9, 51). Further investigation is warranted to understand 332
the mechanism by which Rickettsia reaches and becomes established in these organs and its 333
possible roles there. 334
335
336
ACKNOWLEDGMENTS 337
We thank Eduard Belausov, Vered Holdengreber and Svetlana Kontsedalov for technical 338
assistance. This research was supported by Binational Science Foundation (BSF) grant 2007045, 339
Israel Science Foundation (ISF) grant 884/07. This is contribution number 501/12 from ARO 340
publications. 341
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FIGURE LEGENDS 554
FIG 1 Rickettsia localization in Bemisia tabaci adults by TEM and FISH analysis with 555
Rickettsia-specific probe (blue) and a probe for Portiera (red). (A) Rickettsia occupies most of 556
the body cavity while Portiera is located inside bacteriocytes in the abdomen. (B) Rickettsia is 557
sometimes found at exceptionally high concentrations around the bacteriocytes. (C) Details of 558
the box in (b). (D) TEM image showing three bacteriocytes (B) in the hemolymph surrounded by 559
high concentrations of Rickettsia (R) cells. (E) Rickettsia (R) cells surrounding a bacteriocyte 560
that harbors Portiera (P) and Hamiltonella (H) in the hemolymph of B. tabaci biotype B. (F) Box 561
in E showing a bacteriocyte surrounded by Rickettsia (R) and some Rickettsia-like cells attached 562
to or inside the bacteriocyte. Bar in panel D, 2.5 μm; in panel E, 2 μm and in panel F, 0.5 μm. 563
N, nucleus. 564
565
FIG 2 FISH of Bemisia tabaci ovaries using Rickettsia-specific probe (green), specific probe for 566
Portiera (red) and DAPI staining of the nuclei (blue). (A) Stages 1–4 of ovary development 567
showing very high concentrations of Rickettsia cells invading younger ovaries. (B) One ovary at 568
stage 4 of development showing the distribution of Rickettsia cells in and around it. (C) A focal 569
plane showing the presence of Rickettia cells inside the ovary and at the center of the oocyte (O). 570
(D) Ovary at stage 5 of development showing the included Rickettsia-free bacteriocyte (B). (E) 571
Same as in D with only one focal plane showing Rickettsia cells inside the oocyte. (F) Dissected 572
ovaries and Rickettsia-free bacteriocytes (B) in the hemolymph of Bemisia tabaci. 573
574
FIG 3 TEM sections of Bemisia tabaci abdomen. (A) Stage 1 ovary filled with Rickettsia in 575
follicular cells (FC). (B) Stage 2 ovary filled with and surrounded by Rickettsia (R and arrows). 576
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(C) Stage 3 ovary with follicular cells (FC) and Rickettsia (arrows) mainly in the oocyte (O). (D) 577
Follicular cells (FC) filled with and surrounded by Rickettsia (R and arrows). (E) Mature egg 578
showing the oocyte (O) with Rickettsia excluded and only in the surrounding follicular cells 579
(arrows). H, hemolymph; FV, fat vacuole; FD, fat-dense granules. Bar in panel A, 4 μm; in 580
panel B, 2.5 μm; in panel C, 1 μm ; in panel D, 1 μm; in panel E, 2 μm. 581
582
FIG 4 FISH of dissected midgut using Rickettsia-specific probe (red) and DAPI staining. (A) 583
Whole midgut showing Rickettsia concentrated in clusters in some midgut cells (arrows). (B) 584
DAPI staining showing high concentrations of Rickettsia in the cytoplasm of midgut cells. (C) 585
Same as in B but with FISH using Rickettsia-specific probe showing that the cells stained with 586
DAPI are now labeled with the probe. C, ceca; FC, filter chamber; DM, descending midgut; AM, 587
ascending midgut; H, hindgut; L, lumen; N, nucleus. 588
589
FIG 5 TEM sections of Bemisia tabaci midgut. (A) Concentration of Rickettsia in midgut 590
epithelial cells (EC). (B) Details of the box in A. (C) Concentration of Rickettsia (R) in vacuoles 591
in midgut epithelial cells (EC). (D) Details of the box in C. L, lumen; N, nucleus. Bar in panel A, 592
3 μm; in panel B, 1 μm; in panel C, 2.5 μm ; in panel D, 1 μm. 593
594
FIG 6 TEM section and FISH using Rickettsia-specific probe (green) of Bemisia tabaci primary 595
salivary glands. (A) Two dissected primary salivary glands (PSG) stained with DAPI (blue). (B) 596
Same as in A, with Rickettsia-specific FISH. (C) TEM section in one primary salivary gland 597
(PSG) in the thorax, showing a giant cell and the nucleus (N). (D) Details of box in C showing 598
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Rickettsia-specific FISH in the gland and lipid-like accumulations (arrows). T, thorax; MB, 599
muscle band; R, Rickettsia. Bar in panel C, 2.5 μm; in panel D, 1 μm. 600
601
FIG 7 FISH of Bemisia tabaci stylet using Rickettsia-specific probe (red). Specific FISH signal 602
seen under bright field (A) and dark field (B) in the maxilla that form the food and salivary 603
canals (MX), and in the mandibles (MD) that were detached from the maxilla in this preparation. 604
LR, labrum. 605
606
FIG 8 FISH of Bemisia tabaci testes and spermathecae dissected from males and females, with 607
Rickettsia-specific probe (green) and DAPI staining (blue). (A) Two testicle (T) and two 608
accessory glands (AG) in the male genitalia dissected and stained with DAPI. The ducts 609
connecting the testicles to the common duct (CD) are also seen (arrows). (B) One testicle under 610
bright field showing the major locations of sperm production where the spermatogonia (sg), 611
spermatocytes (sy) and spermatids (st) or mature sperm are located. (C) The same testicle as in B 612
with Rickettsia-specific FISH (green) and DAPI staining. (D) The same testicle as in B and C 613
with Rickettsia-specific FISH only. (E) Spermatheca dissected from fertilized female showing 614
the sperm and Rickettsia-specific FISH (green). (F) Spermatheca seen in E with Rickettsia-615
specific FISH (green) only. 616
617
FIG 9 TEM section in Bemisia tabaci thorax and fat body in the hemolymph. (A) Rickettsia cells 618
(R) are located in one muscle cell close to the nucleus. (B) Several fat body cells (FB) filled with 619
fat vacuoles. (C) Details of the box in B showing Rickettsia cells in fat body cells (arrows). MB, 620
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muscle bands; N, nucleus; FV, fat vacuole. Bar in panel A, 1 μm; in panel B, 2.5 μm; in panel 621
C, 1 μm. 622
623
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