Endogenous viruses form an important proportion of eukaryote genomes and a source of novel functions. How large DNA viruses integrated into a genome evolve when they confer a benefit to their host, however, remains unknown. Bracoviruses are essential for the parasitism success of parasitoid wasps, into whose genomes they integrated ~103 million years ago. Here we show, from the assembly of a parasitoid wasp genome at a chromosomal scale, that bracovirus genes colonized all ten chromosomes of Cotesia congregata. Most form clusters of genes involved in particle production or parasitism success. Genomic comparison with another wasp, Microplitis demolitor, revealed that these clusters were already established ~53 mya and thus belong to remarkably stable genomic structures, the architectures of which are evolutionary constrained. Transcriptomic analyses highlight temporal synchronization of viral gene expression without resulting in immune gene induction, suggesting that no conflicts remain between ancient symbiotic partners when benefits to them converge.
Cotesia wasps (Hymenoptera, Braconidae) are parasitoids of Lepidoptera widely used as biological control agents to control insect pests1,2. Female wasps lay their eggs into caterpillars and larvae develop feeding on the host hemolymph. Parasitoid wasps evolved several strategies that increase parasitic success, including a sensitive olfactory apparatus to locate their hosts3,4 and detoxification mechanisms against plant toxic compounds accumulating in their host (Fig. 1). However, the most original strategy is the domestication of a bracovirus (BV) shared by over 46,000 braconid wasp species5. Bracoviruses originate from a single integration event ~103 million years ago (mya) of a nudivirus (virus having a large DNA genome closely related to well-known baculoviruses) in the genome of the last common ancestor of this group6,7,8,9,10. Virus domestication confers a benefit to the wasps that use BVs as virulence gene delivery systems5. Indeed, virulence genes are introduced with wasp eggs into their hosts, causing inhibition of host immune defenses5,11,12.
To gain insights into the evolution of endogenous viral sequences in the wasp genomes, we obtained a reference genome for Cotesia congregata at a chromosomal scale. Whereas endogenous viruses most often slowly decay after integration13, we show that viral sequences colonized all the chromosomes, reaching a ~2.5-fold higher number of genes than a pathogenic nudivirus. However, the bracovirus is only partially dispersed across the wasp genome since specialized regions of up to two megabases are devoted to the production of packaged DNA and of viral structural proteins. Comparison with genome scaffolds of another wasp revealed a striking stability of these regions over 53 million years14, suggesting strong evolutionary constraints. Expression patterns and molecular evolution of virus genes point to a central role of the viral RNA polymerase in maintaining the bracovirus as a domesticated but still identifiable viral entity. Despite massive virus particle production, wasp immune genes are not induced, suggesting no conflicts remain between the wasp and the virus.
Genome assembly, annotation, and comparison
We used a hybrid sequencing approach combining 454 reads, Illumina short reads, and chromosomal contact data (HiC), to obtain a reference genome for Cotesia congregata at a chromosomal scale. First, a 207 Mb high-quality genome (contig N50 = 48.6 kb, scaffolds N50 = 1.1 Mb and N90 = 65 kb) was obtained for C. congregata using a combination of mate pair 454 pyrosequencing and Illumina sequencing (Supplementary Data 1). Most of the assembly (86%) consisted of 285 scaffolds of over 100 kb. This genome was then reassembled based on experimentally obtained chromosomal contact maps. The HiC method yielded ten main scaffolds comprising >99% of the previously obtained genome assembly (Supplementary Data 1 and Supplementary Fig. 1), and corresponding to the ten chromosomes of C. congregata15 (Supplementary Fig. 1). In addition, draft genomes of five related Cotesia species—C. rubecula, C. glomerata, C. vestalis, C. flavipes, and C. sesamiae—were sequenced and assembled with Illumina shotgun sequencing reads (Supplementary Data 1) for molecular evolution analyses on homologous genes. They respectively resulted in contig N50 values of 13, 9, 15, 20, and 26 kb and cumulative sizes of 216, 243, 176, 155, and 166 Mb.
The genome of C. congregata comprises 48.7% of repeated DNA sequences including 34.7% of known transposable elements (TEs) (Supplementary Fig. 2). Bracovirus proviral segments included TE sequences that had previously been annotated as bracovirus genes: we revealed that the BV26 gene family corresponded to miniature inverted-repeat transposable elements (MITE) derived from Sola2 elements abundant in the wasp genome (Supplementary Fig. 2). This indicates that, contrary to a common paradigm16, the virulence genes packaged in bracovirus particles do not exclusively originate from the wasp cellular gene repertoire.
We automatically annotated 14,140 genes in the genome of C. congregata (Methods and Supplementary Data 1), which include >99% of 1658 conserved insect genes (98 to 99% of the genes for the other Cotesia species, Supplementary Data 1). Then wasp genes potentially involved in the success of the endoparasitoid lifestyle, such as genes implicated in olfaction, detoxification and immunity, were individually annotated. This analysis performed on complex genes belonging to well-known families further assessed the quality of the genome obtained.
Olfaction: highly dynamic evolution of olfactory receptors
Manual annotation of chemoreceptor gene families identified 243 odorant receptor (OR), 54 gustatory receptor (GR), and 105 ionotropic receptor (IR) genes in C. congregata. These numbers are in the upper range of those of other parasitoid wasps, only slightly lower than in ants (Supplementary Data 2), whose large repertoires are attributed to the exploitation of complex ecological niches17. Phylogenetic analyses showed C. congregata ORs belong to 15 of the 18 OR lineages (Fig. 2) described in Apocrita18 and revealed independent OR gene expansions in N. vitripennis and in the Braconidae (Fig. 2). The most spectacular Braconidae-specific expansions occurred in five clades each harboring at least 25 genes in C. congregata (Fig. 2 and Supplementary Data 2). Highly duplicated OR genes were found in 6 clusters of at least 10, and up to 19, tandemly arrayed genes (Supplementary Fig. 3). Within Braconidae, many duplications occurred in the ancestors of Cotesia, but OR copy numbers varied significantly between species (Fig. 2). This illustrates the highly dynamic evolution of OR gene families within parasitoid wasps and between Cotesia species, which have different host ranges. Although the link between genes and adaptation might be complex, this dynamic might be related to host search through the recognition of different volatile compound from insects and plants.
Detoxification genes: a full set but no particular extension
Genes from all families involved in detoxification in insects were identified by manual annotation in C. congregata, and are largely conserved within Cotesia (Supplementary Data 2). For instance, each species harbors conserved numbers of UDP-glucosyltransferases (UGTs) and slightly different numbers of gluthatione-S-transferases (GSTs). In contrast, carboxylesterases (CCEs) and cytochrome P450 (P450s) numbers vary widely with C. flavipes and C. sesamiae harboring few representatives (respectively, 22–24 CCEs and 49 P450s), compared to the 32 CCEs of C. rubecula and the 70 P450s found in C. congregata, which are both exposed to plant toxic compounds (Supplementary Data 2). Cotesia-specific P450 families were identified in the clan 3 and 4, both of which are often associated to adaptation to plant compounds and insecticides19 (Supplementary Data 2). Altogether, Cotesia appear fully equipped for detoxification; however, in contrast to the OR genes, no spectacular gene expansion was observed. This suggests exposure to plant toxic products could be lower than expected on this third trophic level.
Extension of bracovirus in wasp genome
Imbedded in wasp DNA, the virus genomes have been extensively rearranged20 since nudivirus integration. BV sequences (Fig. 1) are differentiated as (i) genes involved in particle production and named “nudiviral” genes (based on clear phylogenetic relationship within the Nudiviridae) and (ii) proviral segments packaged as dsDNA circles in viral particles20, encoding virulence genes which are involved in successful parasitism, and are similar to insect genes21 or specific to bracoviruses20.
The complete genome annotation of C. congregata revealed 102 nudiviral gene copies that have colonized all ten chromosomes. This number is similar to that of pathogenic nudiviruses22, an unexpected result given that endogenous viral elements usually undergo gene loss in the course of evolution, with the exception of genes conferring protection against infections from related viruses13. Here, this surprisingly high number of nudiviral genes results from the balance between gene losses and the expansions of certain gene families. At least 25 of the 32 nudivirus core genes involved in essential viral functions23 have been retained in the wasp genome, with the notable absence of the nudiviral DNA polymerase (Supplementary Fig. 5). The fen genes, generally involved in DNA replication, form a gene family with six tandem copies that is found specifically in the Cotesia lineage (Fig. 3B). The most spectacular expansion, comparable to those of OR genes, concerns the odv-e66 gene family, which is typically found in one or two copies in nudivirus genomes22, but is present as 36 genes in 10 locations (Figs. 2B and 3C), including 6 clusters of 2 to 10 copies, in C. congregata. This expansion occurred both before and after the divergence between C. congregata and M. demolitor24,25, since we found tandemly duplicated copies in homologous loci of both species or in C. congregata only (Fig. 3D). In baculoviruses, odv-e66 encodes a viral chondroitinase26 involved in digesting the peritrophic membrane lining the gut, thus allowing access to target cells during primary infection. We hypothesize that different ODV-E66 proteins may similarly allow BVs to cross various host barriers, and BV infection to spread to virtually all Lepidoptera tissues27,28, thus differing from baculoviruses, whose primary infection is restricted to the gut and rely on a particular virion phenotype (“budded virus”) to spread within their host. The large and continuous odv-e66 gene family expansion we unravel here has most likely played an important role in wasp adaptation. One might speculate that during host shifts of the wasp, bracovirus particles might encounter different barriers, which would require adaptation by competitive evolution of duplicated odv-e66 gene copies in a gene for gene coevolutionary framework29.
Genomic architecture and synteny of bracovirus genes
Chromosome scale genome assembly of C. congregata provides for the first time the comprehensive genomic organization of a bracovirus within the genome of a wasp, allowing us to assess whether nudiviral genes24 and proviral loci20,21 that were previously found in different genome scaffolds could nevertheless be localized in the same chromosomal region. Examination of the very precise map of viral sequences within chromosomes (Fig. 3A, C, E) reveals a complex picture, since bracovirus sequences (nudiviral plus virulence genes) are indeed dispersed and present in all the chromosomes; however, the vast majority of them are organized in clusters. Half of the single-copy nudiviral genes are located in the ~100 Kb nudiviral cluster, which comprises 25 genes (Supplementary Fig. 7). Comparison with the scaffold of M. demolitor showed almost perfect gene content and gene order conservation, as well as conserved syntenic blocks in the genomic regions flanking nudiviral sequences, over ~53 million years of evolution (Fig. 3B). This confirms that the nudiviral clusters of both species are orthologous and likely derive from a genome fragment of the nudivirus that originally integrated in the ancestor wasp genome. This striking stability suggests that major evolutionary constraints maintain these genes together. The other nudiviral genes are dispersed in the wasp genome, although not evenly, as many more loci are located in the smallest chromosomes (Fig. 3A, C) and only one locus in the 4 largest chromosomes. Orthology with M. demolitor could be identified for 20 nudiviral gene regions (Fig. 3D and Supplementary Fig. 7), indicating they were already dispersed in the last common ancestor of both wasps and have stayed in the same loci. Altogether, this showed that nudivirus gene loss and dispersion occurred during the early period of wasp-bracovirus association (100 to 53 mya).
The expansion of virulence genes is another aspect of wasp genome colonization. In C. congregata, the 249 virulence genes encoded by proviral segments are concentrated in 5 regions of the genome located on three chromosomes; indeed among the eight proviral loci previously described20, several were found localized in the same chromosomal region (PL5-PL8, PL3-PL7, PL2-PL4, Fig. 3E). Moreover, 77% of these genes clustered in a single region, which comprises four physically linked proviral loci (PL10-PL1-PL2-PL4) interspersed by wasp genes (Fig. 3E). This major virulence gene coding region (~2 Mb, 177 genes, 17 segments), which we named “macrolocus”, is impressive since it spans half of chromosome 5 short arm and can be compared in size and gene number to the Major Histocompatibility Complex (MHC, ~4 Mb, ~260 genes)30, which plays a major role in mammalian immunity. Orthology relationships was inferred between the PL1 in C. congregata macrolocus and the largest proviral region (comprising 11 segments) of M. demolitor24 (Fig. 3E, F) but the macrolocus has undergone larger expansion in the Cotesia lineage (producing PL2, PL4, and PL10). Further syntenies were found between 5 isolated proviral loci (Fig. 3F), showing they were also already present in the common ancestor of Cotesia and Microplitis lineages 53 million years ago, and indicating that the global organization of the viral genome in wasp DNA was set up earlier. Overall most of the proviral loci are ancient, except the three localized loci in the long arm of chromosome C9 and C10 (PL3 and PL7, PL9 comprising 20 genes), the sole genuine novelties in the Cotesia lineage that appeared within the last 53 million years (Fig. 3F).
Strong conservation of the bracoviral machinery
The DNA circles packaged in bracovirus particles are produced following the genomic amplification of replication units (RU) that span several proviral segments of PLs31,32. Our detailed genomic analyses of C. congregata data led to the identification of a specific sequence motif at each RU extremity (Fig. 4D and Supplementary Fig. 4B) for both previously described types of amplification, associated with either head-tail or tail-tail/head-head concatemers33 (Fig. 4D and Supplementary Fig. 4B), whereas a motif was previously identified for only one type33. We also confirmed the presence of circularization motifs20,21 on all proviral segments at the origin of packaged circles (Fig. 4D and Supplementary Fig. 4B), indicating the conservation of a single viral mechanism whatever the localization of viral sequences (Fig. 4 and Supplementary Fig. 4).
The conservation of viral functions in wasps over 100 million years of evolution is outstanding. Synonymous to non synonymous substitution ratio analyses on orthologous nudiviral genes in Cotesia showed most nudiviral genes (65 genes among the 79 tested genes) are evolving under stabilizing selection that is, however, less stringent than on the set of conserved insect genes used to assess genome completeness (Fig. 4C and Supplementary Fig. 5). This selection is notably strong for genes involved in viral transcription (dN/dS < 0.08), such as the RNA polymerase subunits (lef-4, lef-8, lef-9, p47), which most likely control nudiviral genes expression and, consequently, bracovirus particle production6,10. In contrast, genes involved in infectivity (homologs of baculovirus pif genes) appear less conserved (Supplementary Fig. 5). This might reflect divergence occurring during host shifts, through adaptation of virus envelope proteins to particular host cell receptors. The large odv-e66 gene family and duplicated genes (p6.9_2, pif-5_2, 17a) similarly displayed less stringent to relaxed selection (Fig. 4 and Supplementary Fig. 5), which might be conducive to mutational space exploration for adaptation by neo-functionalization or sub-functionalization34. Virulence genes encoded by proviral segments globally displayed low conservation (Fig. 4), as expected for genes interacting with host defenses and involved in evolutionary arms race or adaptation to new hosts35.
Synchronized nudiviral transcription precedes bracovirus production
The onset of bracovirus particle production has been detected using molecular biology and transmission electronic microscopy late during metamorphosis, 4 days after larvae have emerged from the caterpillar36. Previous experiments studying a handful of nudiviral genes during C. congregata pupal development showed a strong calyx specificity and unexpectedly early expression of a gene involved in nudiviral transcription6,10. We used RNAseq analysis to assess, for the first time, the expression of the complete set of 102 nudivirus genes in the ovaries throughout pupal development. The aim was to investigate in detail viral gene expression timing and whether nudiviral genes were synchronized. Genes involved in nudiviral transcription are highly expressed at day 2, but unexpectedly a large set of nudiviral genes transcripts is also detected at that time (Fig. 5C). Altogether, these results suggest that the onset of nudiviral gene transcription very quickly follows the production of the viral RNA polymerase, as would typically occur within 12 h in baculovirus infection. Afterwards at day 3, nudivirus gene expression has reached a much higher level, which could reflect that more cells are undergoing virus replication. The level then increased more slowly and reached a maximum at day 5 (Fig. 5, Supplementary Data 4, and Supplementary Fig. 6), when virus particle production is the highest. Genes involved in viral transcription displayed a different pattern, since they already reached high level expression at day 2 and decreased significantly during virus production either from day 4 or day 5 (Fig. 5B). This time shift between expression of transcription and other nudiviral genes supports the hypothesis that the nudiviral RNA polymerase controls the expression of the other viral genes. The gap between nudivirus gene expression (day 2) and the onset of previously determined particle production (day 4) could reflect that very few cells may initially be involved in replication, and thus that high-throughput sequencing is required for their early detection. This hypothesis has important implications for studying how virus production is initially and selectively induced in the ovaries, which remains a major knowledge gap for understanding the wasp-bracovirus relationship.
Although nudiviral gene expression is variable, many transcripts reached impressive levels, similar to what would be expected of regular viral genes during infection. Indeed 12 nudiviral genes are among the top 50 of most expressed genes in C. congregata ovaries at day 5 (Supplementary Data 4). Moreover, three genes from the nudiviral cluster (including the major capsid component vp39) are by far the 3 most expressed of all wasp genes, suggesting virus particle production might mobilize most replicating cells transcription activity.
The analysis of venom gland transcripts, however, revealed some exceptions to nudiviral gene tissue-specificity, since 9 out of the 102 studied nudiviral genes are expressed in the venom gland (Fig. 5B). The fen-3c gene, for example, reached a high level in the venom gland and showed no expression in the ovaries. Moreover, transcripts of some of the gene copies belonging to extended gene families are barely detected in any samples (odve66-31, odve66-35) (Fig. 5B); they may correspond to pseudogenes, or, like fen-3c, be expressed in other tissues, for a new function, no longer related to bracovirus production. For the vast majority of nudiviral genes, however, expression remains strongly synchronized during pupal ovarian development, turning on at day 2 and being already high at day 3 (Fig. 5B). Considering the age of the nudivirus wasp association, this reinforces the idea of strong evolutionary constraints.
Immune gene expression during bracovirus production
After 100 million years of endogenous evolution within the wasp genome, one can question whether virus particles produced massively in the ovaries are considered as a pathogenic virus by the wasp, in which case their production should trigger an immune response. Whether viral production interacts in any way with the wasp immune system has remained totally unknown, however. Globally, the annotation of immune-related genes indicated C. congregata has an arsenal of 258 immune genes that are potentially involved in recognition, signal transduction, different signaling pathways, melanization and effector functions (Supplementary Data 2), in accordance with the recently reported annotation of C. vestalis immune genes37. We identified all members of the Toll, IMD, Jak/STAT and RNA interference pathways found in Hymenoptera (Supplementary Data 2).
In contrast to the sharp increase in nudiviral gene expression, no significant changes in immune gene expression could be detected in the ovaries during pupal development (Fig. 6, Supplementary Data 4, and Supplementary Fig. 6). In particular, expression of the genes involved in antiviral immunity (encoding members of the RNA interference, Jak/STAT or Imd/JNK pathways) was high in ovaries, even at stages before particle production is observable (ovaries stages 2 to 4), but hardly fluctuated during the course of ovary development, even at day 5, when massive particle production becomes apparent by TEM (Fig. 5A). Thus, no immune response appears to be induced or repressed at the cellular level as a response to high level nudiviral gene expression and particle production.
To investigate the genome features related to the endoparasitoid lifestyle of species associated with endogenous bracoviruses, we sequenced the genomes of six Cotesia species, and obtained an assembly at the chromosomal scale for C. congregata. This approach provided insights into genes potentially involved in essential functions of the wasps, such as olfaction, detoxification and immunity, as well as into the genomic evolution of the bracovirus. Large OR gene diversifications are often associated with host localization and acceptance. Indeed, female wasps rely on a sensitive olfactory apparatus to locate their hosts from volatile cues plants emit in response to herbivore attacks3, and to assess caterpillar quality before oviposition38. Interestingly, OR copy numbers varied significantly during the evolution of the genus Cotesia (Fig. 2). The high dynamics of OR repertoire might point to the need for more specific recognition of chemical cues from the host and its food plant. Characterization of OR gene sequences is the first step toward determining their function, and experimental settings using Drosophila cells are available for the identification of the volatile recognized by each receptor. This is of particular interest for future research on the modification of host acceptance through genome editing, to improve parasitoid strains used in biological control.
In contrast, no comparable diversification was observed in the detoxification arsenal, even though Cotesia larvae can be exposed to various toxic phytochemicals while feeding on the hemolymph of caterpillar hosts (e.g., potential exposure of C. congregata to insecticidal nicotine when parasitizing Manduca sexta feeding on tobacco; of C. rubecula, C. glomerata and C. vestalis to glucosinolates by developing in hosts consuming crucifers; and of C. flavipes to phenylpropanoids and flavonoids as parasitizing hosts on sugarcane). This surprisingly low diversification of the detoxification arsenal could suggest that wasp larvae may not be as exposed to toxic compounds as expected due to direct excretion of these chemicals by the host larvae39,40 or to the sequestration of toxic compounds41 in tissues not consumed by parasitoid larvae. It is also possible that some bracovirus virulence genes of unknown function might contribute to protect parasitoid larvae against toxic compounds.
Cotesia wasps face different immune challenges during their lifetimes. While feeding on nectar, the adult might be exposed to similar environmental challenges to honey bees. Development inside the caterpillar host could on the one hand shield wasp larvae from pathogens, but on the other hand expose them to opportunistic infections, because parasitism alters caterpillar immune defenses. Lastly, metamorphosis coincides with the production of bracovirus particles, against which wasp antiviral responses had so far not been investigated. Insects were recently shown to recognize their obligate bacterial symbionts as foreign and to exert strong immune control, as documented for Sitophilus oryzae Primary Endosymbiont (SOPE)42. As the immunity gene arsenal of C. congregata is comparable to that of the honey bee, this wasp is most probably able to mount an immune response against pathogens, including viruses. However, the transcriptomic approach did not reveal any significant difference in immune gene expression between the ovaries of different pupal stages, although massive amounts of bracovirus particles are produced from day 5. This might reflect a lack of ovary cells ability to react, or that virus particles are recognized as self. Whatever the mechanism involved, there is apparently no conflict remaining between the wasp and the virus after this ancient endogenization. We cannot exclude the possibility that immune cells from the hemolymph or fat body could perceive virus particle production and mount an immune response. However, this seems unlikely, since virus producing cells are tightly isolated by an epithelial layer and the ovary sheath: particles have not been observed in other wasp tissues and are not present in the hemolymph, they are exclusively released in the ovary lumen.
With the ancestral integration of a nudivirus genome, the parasitoid wasp gained a series of viral functions: including viral transcription, viral DNA replication, particle morphogenesis and infectivity. Whereas the function of viral DNA replication has been lost5, thus impeding autonomous virus re-emergence, the other viral functions have been reorganized for virulence gene transfer via bracovirus particles. Chromosomal scale resolution of the C. congregata genome showed that bracovirus genes have colonized all the chromosomes with a nearly 2.5-fold increase in the total number of virus genes (nudiviral plus virulence genes) compared to the genome of a pathogenic nudivirus. This contrasts sharply with the decay of most viruses integrated into eukaryote genomes that do not provide a benefit to their host. Bracovirus dispersion occurred between 100 and 53 mya, as 25 viral loci are orthologous between Cotesia and Microplitis (Fig. 3 and Supplementary Fig. 7) and most of the proviral segments were already present in their common ancestor. The genomic organization stasis, observed since then, is reminiscent of bacterial symbiont genomes, which underwent major rearrangements specifically during the initial steps of association43. Yet, the organization of many bracovirus genes in clusters suggests that strong evolutionary constraints maintain these genes together. In the case of the nudiviral cluster, which encodes major capsid components (VP39, 38 K) on chromosome 7, DNA amplification, as a single unit31, might enable mass production of bracoviral particles that are injected into parasitized hosts and accordingly many nudiviral cluster genes are the highest or among the most expressed genes in the ovaries. This could explain the counter selection on the dispersion or loss of these clustered nudivirus genes since the separation of the Cotesia and Microplitis lineages. In the case of the particularly large macrolocus, which comprises 77% of the virulence genes in the Cotesia genome, clustering could facilitate the evolution of new virulence genes copies by duplication20, and thereby wasp adaptation against host resistance or to new hosts5,29. This organization may also promote the transmission of bracovirus virulence genes as a block of co-evolved genes, as shown for supergenes involved in butterfly wing patterns44 and ant social behavior45. More generally our study shows that Bracovirus nudiviral cluster and proviral loci belong to remarkable genomic structures, the architecture of which are as evolutionarily constrained as supergenes, ribosomal DNA regions, Major Histocompatibility Complex, and chorion genes clusters. The next challenge will be to determine whether proximal causes are also underlying this organization as for example by further dissecting bracovirus DNA replication mechanism and identifying the role of the conserved regulatory signals we found at all replication unit extremities.
Remarkably, despite their semi-dispersed locations in the wasp genome, nudiviral genes remain synchronically expressed and under stabilizing selection, thus enabling the production of infectious bracovirus particles. This striking conservation of the viral machinery highlights the paramount importance of the production of viral particles allowing virulence gene transfer to a host, in the evolutionary history of the wasp. Strikingly, the stability of bracovirus loci in the wasp genome over 53 million years is in sharp contrast with recently reported high mobility of endogenous Ichnoviruses (IVs), which evolved within ichneumonid wasp genomes from a different virus ancestor46. This difference might reflect characteristic features of the originally integrated virus, such as an ability to transpose, that could impact the evolution of viral sequences within wasp genomes. As an alternative hypothesis, IVs, contrary to BVs, may have not reached the stage leading to stabilization of viral loci in the wasp genome; indeed it is not known whether a single ancient or several recent endogenization events of viruses from the same family occurred in ichneumonid wasps46. In addition to IVs and BVs, several independent events of nudivirus captures have led to the production of viral liposomes allowing the delivery of virulence proteins to the parasitized host instead of virulence genes47,48,49,50,51. Comparisons between high-quality genomes of a variety of parasitoid wasps convergently associated with different viruses would be essential to reveal whether the evolution of beneficial large DNA endogenous viruses follows universal rules or each time a unique trajectory.
Materials and methods
The C. congregata laboratory strain was reared on its natural host, the tobacco hornworm, M. sexta (Lepidoptera: Sphingidae) fed using artificial diet containing nicotine as previously described20. C. sesamiae isofemale line came from individuals collected in the field in Kenya (near the city of Kitale) and was maintained on Sesamia nonagrioides52. C. flavipes individuals originated from the strain used for biological control against Diatraea saccharalis in Brazil53. C. glomerata, C. rubecula and C. vestalis laboratory cultures were established from individuals collected in the vicinity of Wageningen in Netherlands, and reared on Pieris brassicae, Pieris rapae, and Plutella xylostella larvae, respectively54,55. To reduce the genetic diversity of the samples prior to genome sequencing, a limited number of wasps were pooled; for example, only haploid males from a single virgin female were used for Illumina sequencing of C. congregata genome, ten female and male pupae originating from a single parent couple were used to generate C. glomerata genome, five male pupae originating from a single C. rubecula virgin female for C. rubecula genome and 40 adult males and 8 adult females from multiple generations of C. vestalis cultured in the Netherlands were used. DNAs were extracted from adult wasps and stored in extraction buffer following two protocols. C. congregata, C. sesamiae and C. flavipes DNA were extracted using a Qiamp DNA extraction kit (Qiagen) with RNAse treatment following the manufacturer’s instructions and eluted in 200 µl of molecular biology grade water (5PRIME). C. glomerata, C. rubecula and C. vestalis DNA was extracted using phenol-chloroform.
Genome sequencing and assembly
Cotesia congregata genome was sequenced combining two approaches: (i) single-end reads and MatePair libraries of 3 Kb, 8 Kb, and 20 Kb fragments on 454 GS FLX Titanium platform (Roche) and (ii) paired-end reads of 320 bp fragments with HiSeq2000 platform (Illumina). C. glomerata, C. rubecula and C. vestalis DNA libraries were prepared using insert sizes of 300 and 700 bp. For C. sesamiae and C. flavipes libraries an insert size of 400 bp was selected. These libraries were sequenced in 100 bp paired-end reads on a HiSeq2000 platform (Illumina) at the French National Sequencing Institute (CEA/Genoscope, France) and at the Sequencing Facility of the University Medical Center (Groningen, Netherlands). Reads were then filtered according to different criteria: low-quality bases (Q < 20) at the read extremities, bases after the second N found in a read, read shorter than 30 bp and reads matching with phiX (Illumina intern control) were removed using in-house software (http://www.genoscope.cns.fr/fastxtend) based on the FASTX-Toolkit (http://hannonlab.cshl.edu/fastx_toolkit) as described in ref. 56.
The C. congregata genome was generated by de novo assembly of 454 reads using GS De Novo Assembler from the Newbler software package v2.857. The consensus was polished using the Illumina data as previously described58. Gaps were filled using GapCloser module from the SOAPdenovo assembler59. The genomes of C. sesamiae, C. flavipes, C. glomerata, C. rubecula and C. vestalis were assembled with Velvet v1.2.0757 using the following parameters: velveth k-mer 91 -shortPaired -fastq -separate, velvetg -clean yes and specific adapted values for -exp_cov and -cov_cutoff for each species.
Chromosome scale assembly of C. congregata genome
Hi-C library preparation
The individual wasps had their gut removed and were immediately suspended after sampling in 30 mL of 1X tris-EDTA buffer and formaldehyde at 3% concentration, then fixed for 1 h. Ten milliliters of glycine at 2.5 M was added to the mix for quenching during 20 min. A centrifugation recovered the resulting pellet for −80 °C storage and awaiting further use. The libraries were then prepared and sequenced (2 × 75 bp, paired-end Illumina NextSeq with the first ten bases acting as tags), as previously described60 using the DpnII enzyme.
Read processing and Hi-C map generation
The Hi-C read library was processed and mapped onto DpnII fragments of the reference assembly using HiCbox (available at https://github.com/rkoszul/HiC-Box) with bowtie261 on the back-end (option --very-sensitive-local, discarding alignments with mapping quality below 30). Fragments were then filtered according to size and coverage distribution, discarding sequences shorter than 50 bp or below one standard deviation away from the mean coverage. Both trimmed contact maps were then recursively sum-pooled four times by groups of three, yielding bins of 34 = 81 fragments.
The genome was reassembled using an updated version of GRAAL (dubbed instaGRAAL62) for large genomes on the aforementioned contact maps for 1000 cycles, as described62. Briefly, the program modifies the relative positions and/or orientations of sequences according to expected contacts given by a polymer model. These modifications take the form of a fixed set of operations (swapping, flipping, inserting, merging, etc.) on the 81-fragment bins. The likelihood of the model is maximized by sampling the parameters with a Markov Chain Monte Carlo (MCMC) method. After a number of iterations, the contact distribution converges and the global genome structure ceases to evolve, at which point the genome is considered reassembled. The process yielded eleven main scaffolds comprising >99% of the bin sequences.
Polishing and post-assembly processing
Each scaffold was independently polished by reconstructing the initial contig structure whenever relocations or inversions were found. In addition, previously filtered sequences were reintegrated next to their original neighbors in their initial contig when applicable. The implementation is part of instaGRAAL polishing and available at https://github.com/koszullab/instaGRAAL (run using the –polishing mode).
We performed the validation with QUAST-LG63, an updated version of the QUAST analyzer tailored for large genomes. The initial assembly from Illumina short reads was used as reference. The assessed metrics include genomic feature completeness, Nx and NGx statistics as well as global and local misassemblies. In addition, each assembly was assessed for ortholog completeness with BUSCO v364. The reference dataset used for expected gene content was pulled from the OrthoDB (version 9) database for Hymenoptera, comprising 4,415 orthologs.
Transposable element annotation
Genome annotation was first done on the C. congregata reference genome and then exported on the genomes of the five other Cotesia species. First, the transposable element annotation was realized following the REPET pipeline comprising a de novo prediction (TEdenovo) and an annotation using TE libraries (TEannot)65. This annotation was exported into GFF3 files used as mask for the gene annotation.
Automated gene annotation
The automated gene prediction and annotation of C. congregata genome was done using Gmove (https://github.com/institut-de-genomique/Gmove) integrating different features based on (i) the mapping of Hymenoptera proteins from all hymenopteran genomes available on NCBI and UniProt Hymenoptera, (ii) the mapping of RNA-Seq data from C. congregata, C. glomerata, C. vestalis, and C. rubecula (this paper and PRJNA289655, PRJNA485865 PRJNA289731), and (iii) ab initio genes predictions using SNAP66. The automated annotation of the five other Cotesia species was performed using MAKER67 using the same features as for the annotation of C. congregata but also including the output automated annotation of C. congregata.
Automated gene functional annotation
The functional annotation was performed using blastp from BLAST + v2.5.068 to compare the C. congregata proteins to the NCBI nonredundant database (from the 29/06/2014). The ten best hits below an e-value of 1e-08 without complexity masking were conserved. Interproscan v5.13-52.069 was used to analyze protein sequences seeking for known protein domains in the different databases available in Interproscan. Finally, we used Blast2GO70 to associate a protein with a GO group (Supplementary Fig. 8).
Specialist gene annotation
The automated annotations were followed by manual curations, corrections and annotations realized by specialists of each gene family of interest through Apollo71. The genomes were available to this consortium through the web portal: https://bipaa.genouest.org/is/parwaspdb. Supplementary Data 2 summarizes the genes manually annotated by experts of different biological functions according to the phylogenetic level of interest for the comparisons. For the study of Cotesia immunity it was interesting to verify manually those of C. congregata genome to study whether they were induced after bracovirus particles production, the immune genes of other species were only automatically annotated.
Genome completeness evaluation
The completeness of the genomes and annotations were evaluated using Benchmarking Universal Single-Copy Orthologs BUSCO v364 using the insecta_odb9 database composed of 1658 genes. Contigs were searched for similarities against the nonredundant NCBI nucleotide (nt) (release November 2019) and the Uniref90 protein (release November 2019) databases using, respectively, blastn from BLAST + v2.7.168 and diamond v0.9.29.13072. For both tasks, e-value cutoff was set to 10−25. Taxa were inferred according to the highest-scoring matches sum across all hits for each taxonomic rank in the two databases. Sequencing coverage was deduced after mapping Illumina paired reads to the assembly with Bowtie2 v188.8.131.521. Contigs were then displayed with Blobtools v1.1.173 using taxon-annotated-GC-coverage plots.
Orthologous genes identification, alignment, and phylogeny
Orthologous genes between all genes annotated in the six Cotesia species and the four outgroups (Microplitis demolitor, Nasonia vitripennis, Apis mellifera and Drosophila melanogaster) were identified using OrthoFinder v1.1474. Universal single-copy ortholog genes from BUSCO v364 were extracted for the six Cotesia species and the four outgroups, aligned using MAFFT v7.01775 and concatenated. The species phylogeny was performed on this alignment composed of 1058 orthologous for a length of 611 kb using PhyML program76 with the HKY85 substitution model, previously determined by jModelTest v2.177 and the branch support were measured after 1000 bootstrap iterations. The cluster of orthologous genes was used to determine the phylogenetic level of each gene represented in Fig. 2. as follows: genes shared by all species are called shared by all; genes shared by at least nine species among the ten studied species without phylogenetic logical are named “shared by some”; genes shared by only Hymenoptera species and without orthologous gene in D. melanogaster are considered as “Hymenoptera specific”; genes shared only by Microgastrinae are named “Microgastrinae specific”; genes shared only by Cotesia species and without orthologous genes in any of the outgroup are considered as “Cotesia specific”.
The different synteny analyses were performed on the orthologous genes identified by OrthoFinder v1.1474 and by reciprocal blastp from BLAST + v2.2.28 on the annotated proteins (e-value below 10e−20). The correspondence between the genes, the localizations on the scaffold and the figures were realized thanks to a custom R script (R Core Team 2013).
Evolution of gene families
For OR, P450 and odv-e66 genes manually annotated genes from the reference genome of C. congregata were used along with orthologous genes from the five other Cotesia species, M. demolitor78, N. vitripennis79, A. mellifera80 to create a phylogeny of each family among Hymenoptera. Protein sequences were first aligned with MAFFT v7.01775 and the maximum-likelihood phylogeny was performed with PhyML76 using the JTT + G + F substitution model for OR and using HKY80 substitution model for P450 and odv-e66 genes. The branch support was assessed using aLRT for OR and 1000 bootstraps for P450 and odv-e66 genes. The trees were then rooted to Orco (OR-coreceptor) clade for OR and the midpoint for the other. The gene gains and losses along the phylogeny for the different gene families of interest were identified with NOTUNG v2.981 as described82.
Evolution of single-copy genes
To determine evolutionary rates within Cotesia genus, single-copy orthologous gene clusters (BUSCO, nudiviral and virulence genes) were first aligned using MACSE83 to produce reliable codon-based alignments. From these codon alignments, pairwise dN/dS values were estimated between C. congregata and C. sesamiae, the two most diverging species in the Cotesia phylogeny, with PAML v4.884 using the YN00 program. dN/dS of the different gene categories of interest were then compared using a Kruskal–Wallis test, and Nemenyi-Tests for multiple comparisons were realized with the R package. For the nudiviral genes the dN/dS values were calculated using genes from the six species. Orthologous genes from the six Cotesia species were aligned as described before and codeml (implemented in PAML v4.8) was used to estimate the M0 dN/dS (free ratio model). This model was compared to a neutral model for which the dN/dS is fixed to 1.
Sample preparation, extraction, and sequencing
The ovaries and venom glands were extracted from females at five pupal stages, i.e., days 2, days 3, days 4, days 5 and at emergence, corresponding to the number of days after the creation of the cocoon and identified following body melanization36. Ovaries were pooled by groups of 20 pairs and venom glands by 100 and in duplicates for each condition. Samples were stored in buffer provided in the extraction kit by adding β-mercaptoethanol to reduce RNA degradation. Extractions were performed using QIAGEN RNeasy kit following manufacturer’s recommendations. RNA-Seq library preparations were carried out from 1 to 2 µg total RNA using the TruSeq Stranded mRNA sample prep kit (Illumina, San Diego, CA, USA), which allows mRNA strand orientation (sequence reads occur in the same orientation as anti-sense RNA). Briefly, poly(A) + RNA was selected with oligo(dT) beads, chemically fragmented and converted into single-stranded complementary DNA (cDNA) using random hexamer priming. Then, the second strand was generated to create double-stranded cDNA. cDNA were then 3’-adenylated, and Illumina adapters were added. Ligation products were PCR-amplified. Ready-to-sequence Illumina libraries were then quantified by qPCR using the KAPA Library Quantification Kit for Illumina Libraries (KapaBiosystems, Wilmington, MA, USA), and libraries profiles evaluated with an Agilent 2100 Bioanalyzer (Agilent Technologies, Santa Clara, CA, USA). Each library was sequenced using 101 bp paired-end reads chemistry on a HiSeq2000 Illumina sequencer.
The pair-end reads from C. congregata ovary and venom gland libraries were mapped on the reference genome using TopHat285 with default parameters. Then, featureCounts program from the Subread package86 was used to determine fragment counts per genes using default parameters.
To analyze gene expression, the raw fragment counts of ovaries and venom glands samples were first converted to counts per million (CPM) using the edgeR-implemented package87 (R-Core Team 2017). Expressed genes were filtered based on a CPM > 0.4 (corresponding to raw count of 15) in at least two of the libraries incorporated in the analysis (Supplementary Fig. 9A) and subsequent normalization was performed on CPMs using the edgeR TMM method for Normalization Factor calculation88 (Supplementary Fig. 9B). The reproducibility of replicates was then assessed by Spearman correlation of gene expression profiles based on filtered and normalized CPMs (Supplementary Fig. 9C).
To examine differential expression between ovary stages and with venom glands a quasi-likelihood-negative binomial generalized log-linear model was fitted to the data after estimation of the common dispersion using edgeR. Then, empirical Bayes quasi-likelihood F-tests were performed to identify differentially expressed (DE) genes under chosen contrasts89. Finally, F-test p-values were adjusted using false-discovery rate (FDR) method90. Genes were considered as DE whether FDR < 0.05 and fold-change (FC) of expressions between compared conditions was higher or equal to 1.5. Four contrasts were designed between the five successive ovary stages and a control contrast was tested between ovaries and venom glands at wasp emergence stage.
Statistics and reproducibility
To obtain high-quality genome assemblies it is necessary to limit the variability of the samples used for sequencing, which was done as much as possible for the six Cotesia genomes reported, as described in the sampling section. Access to the variability of these genomes will require resequencing approaches. Different statistical analyses are deeply involved in nearly all steps of the study from genome assemblies to transcriptome analyses and reported in the corresponding sections.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
The datasets and genomes generated during the current study are available from the European Bioinformatic Institute (EMBL-EBI) and National Center for Biotechnology Information (NCBI) at the following BioProject IDs: PRJEB36310 and PRJEB43234 (umbrella project PRJEB40240). Genome database (genomes and annotated genes) is also available on the web site BIPAA (Bioinformatic Platform for Agrosystem Arthropods) https://bipaa.genouest.org/is/parwaspdb/.
Custom scripts are available from https://github.com/JeremyLGauthier/Scripts_Cotesia_Genomes or on Zenodo doi: 10.5281/zenodo.411641291.
Parra, J. R. P. biological control in Brazil: an overview. Sci. Agric. 71, 420–429 (2014).
Parra, J. R. P. & Coelho, A. Applied biological control in Brazil: from laboratory assays to field application. J. Insect Sci. 19, 1–6 (2019).
Dicke, M. Behavioural and community ecology of plants that cry for help. Plant Cell Env. 32, 654–666 (2009).
Poelman, E. H. et al. Hyperparasitoids use herbivore-induced plant volatiles to locate their parasitoid host. PLoS Biol. 10, e1001435 (2012).
Gauthier, J., Drezen, J. M. & Herniou, E. A. The recurrent domestication of viruses: major evolutionary transitions in parasitic wasps. Parasitology 145, 713–723 (2018).
Bézier, A. et al. Polydnaviruses of braconid wasps derive from an ancestral nudivirus. Science 323, 926–930 (2009).
Thézé, J., Bézier, A., Periquet, G., Drezen, J. M. & Herniou, E. A. Paleozoic origin of insect large dsDNA viruses. Proc. Natl Acad. Sci. USA 108, 15931–15935 (2011).
Drezen, J.-M., Herniou, E. A. & Bézier, A. in Parasitoid Viruses Symbionts and Pathogens (eds Beckage, N. E. & Drezen, J.-M.) 15–31 (Elsevier, San Diego, 2012).
Burke, G. R. & Strand, M. R. Deep sequencing identifies viral and wasp genes with potential roles in replication of Microplitis demolitor Bracovirus. J. Virol. 86, 3293–3306 (2012).
Burke, G. R., Thomas, S. A., Eum, J. H. & Strand, M. R. Mutualistic polydnaviruses share essential replication gene functions with pathogenic ancestors. PLoS Pathog. 9, e1003348 (2013).
Beckage, N. E., Tan, F., Schleifer, K. W., Lane, R. D. & Cherubin, L. L. Characterization and biological effects of Cotesia congregata polydnavirus on host larvae of the tobacco hornworm, Manduca sexta. Arch. Insect Biochem. Physiol. 26, 165–195 (1994).
Strand, M. R. in Parasitoid Viruses Symbionts and Pathogens (eds Beckage, N. E. & Drezen, J.-M.) 149–161 (Elsevier, San Diego, 2012).
Katzourakis, A. & Gifford, R. J. Endogenous viral elements in animal genomes. PLoS Genet. 6, e1001191 (2010).
Murphy, N., Banks, J. C., Whitfield, J. B. & Austin, A. D. Phylogeny of the parasitic microgastroid subfamilies (Hymenoptera: Braconidae) based on sequence data from seven genes, with an improved time estimate of the origin of the lineage. Mol. Phylogenet. Evol. 47, 378–395 (2008).
Belle, E. et al. Visualization of polydnavirus sequences in a parasitoid wasp chromosome. J. Virol. 76, 5793–5796 (2002).
Gundersen-Rindal, D., Dupuy, C., Huguet, E. & Drezen, J.-M. Parasitoid polydnaviruses: evolution, pathology and applications. Biocont. Sci. Technol. 23, 1–61 (2013).
Robertson, H. M. Molecular evolution of the major arthropod chemoreceptor gene families. Ann. Rev. Entomol. 64, 227–242 (2019).
Zhou, X. et al. Phylogenetic and transcriptomic analysis of chemosensory receptors in a pair of divergent ant species reveals sex-specific signatures of odor coding. PLoS Genet. 8, e1002930 (2012).
Wang, H. et al. CYP6AE gene cluster knockout in Helicoverpa armigera reveals role in detoxification of phytochemicals and insecticides. Nat. Commun. 9, 4820 (2018).
Bézier, A. et al. Functional endogenous viral elements in the genome of the parasitoid wasp Cotesia congregata: insights into the evolutionary dynamics of bracoviruses. Philos. Trans. R. Soc. B 368, 0047 (2013).
Desjardins, C. A. et al. Comparative genomics of mutualistic viruses of Glyptapanteles parasitic wasps. Genome Biol. 9, R183 (2008).
Bézier, A. et al. The genome of the nucleopolyhedrosis-causing virus from Tipula oleracea sheds new light on the Nudiviridae family. J. Virol. 89, 3008–3025 (2015).
Harrison, R. L. et al. ICTV virus taxonomy profile: nudiviridae. J. Gen. Virol. 101, 3–4 (2020).
Burke, G. R., Walden, K. K., Whitfield, J. B., Robertson, H. M. & Strand, M. R. Widespread genome reorganization of an obligate virus mutualist. PLoS Genet. 10, e1004660 (2014).
Burke, G. R., Walden, K. K. O., Whitfield, J. B., Robertson, H. M. & Strand, M. R. Whole genome sequence of the parasitoid wasp Microplitis demolitor that harbors an endogenous virus mutualist. G3 (Bethesda) 8, 2875–2880 (2018).
Sugiura, N. et al. Chondroitinase from baculovirus Bombyx mori nucleopolyhedrovirus and chondroitin sulfate from silkworm Bombyx mori. Glycobiology 23, 1520–1530 (2013).
Wyder, S., Blank, F. & Lanzrein, B. Fate of polydnavirus DNA of the egg-larval parasitoid Chelonus inanitus in the host Spodoptera littoralis. J. Insect Physiol. 49, 491–500 (2003).
Beck, M. H., Inman, R. B. & Strand, M. R. Microplitis demolitor bracovirus genome segments vary in abundance and are individually packaged in virions. Virology 359, 179–189 (2007).
Herniou, E. A. et al. When parasitc wasps hijacked viruses: genomic and functionnal evolution of polydnaviruses. Philos. Transac. R. Soc. B 368, 1–13 (2013).
Trowsdale, J. & Knight, J. C. Major histocompatibility complex genomics and human disease. Annu. Rev. Genomics Hum. Genet. 14, 301–323 (2013).
Louis, F. et al. The bracovirus genome of the parasitoid wasp Cotesia congregata is amplified within 13 replication units, including sequences not packaged in the particles. J. Virol. 87, 9649–9660 (2013).
Drezen, J. M., Chevignon, G., Louis, F. & Huguet, E. Origin and evolution of symbiotic viruses associated with parasitoid wasps. Cur. Opin. Insect Sci. 6, 35–43 (2014).
Burke, G. R., Simmonds, T. J., Thomas, S. A. & Strand, M. R. Microplitis demolitor bracovirus proviral loci and clustered replication genes exhibit distinct DNA amplification patterns during replication. J. Virol. 89, 9511–9523 (2015).
Francino, M. P. An adaptive radiation model for the origin of new gene functions. Nat. Genet. 37, 573–577 (2005).
Gauthier, J. et al. Genetic footprints of adaptive divergence in the bracovirus of Cotesia sesamiae identified by targeted resequencing. Mol. Ecol. 27, 2109–2123 (2018).
Pasquier-Barre, F. et al. Polydnavirus replication: the EP1 segment of the parasitoid wasp Cotesia congregata is amplified within a larger precursor molecule. J. Gen. Virol. 83, 2035–2045 (2002).
Shi, M. et al. The genomes of two parasitic wasps that parasitize the diamondback moth. BMC Genomics 20, 893 (2019).
Bichang’a, G. et al. Alpha-amylase mediates host acceptance in the Braconid parasitoid Cotesia flavipes. J. Chem. Ecol. 44, 1030–1039 (2018).
Kumar, P., Pandit, S. S., Steppuhn, A. & Baldwin, I. T. Natural history-driven, plant-mediated RNAi-based study reveals CYP6B46’s role in a nicotine-mediated antipredator herbivore defense. Proc. Natl Acad. Sci. USA 111, 1245–1252 (2014).
Pentzold, S. et al. Metabolism, excretion and avoidance of cyanogenic glucosides in insects with different feeding specialisations. Insect Biochem. Mol. Biol. 66, 119–128 (2015).
Petschenka, G. & Agrawal, A. A. How herbivores coopt plant defenses: natural selection, specialization, and sequestration. Curr. Opin. Insect Sci. 14, 17–24 (2016).
Masson, F., Zaidman-Remy, A. & Heddi, A. Antimicrobial peptides and cell processes tracking endosymbiont dynamics. Phil. Trans. Royal Soc. B 371, 20150298 (2016).
Moran, N. A. & Mira, A. The process of genome shrinkage in the obligate symbiont Buchnera aphidicola. Genome Biol. 2, 1–12 (2001).
Joron, M. et al. Chromosomal rearrangements maintain a polymorphic supergene controlling butterfly mimicry. Nature 477, 203–206 (2011).
Wang, J. et al. A Y-like social chromosome causes alternative colony organization in fire ants. Nature 493, 664–668 (2013).
Legeai, F. et al. Genomic architecture of endogenous ichnoviruses reveals distinct evolutionary pathways leading to virus domestication in parasitic wasps. BMC Biol. 18, 89 (2020).
Pichon, A. et al. Recurrent DNA virus domestication leading to different parasite virulence strategies. Sci. Adv. 1, e1501150 (2015).
Drezen, J. M. et al. Endogenous viruses of parasitic wasps: variations on a common theme. Curr. Opin. Virol. 25, 41–48 (2017).
Leobold, M. et al. The Domestication of a large DNA virus by the wasp Venturia canescens involves targeted genome reduction through pseudogenization. Genome Biol. Evol. 10, 1745–1764 (2018).
Burke, G. R., Simmonds, T. J., Sharanowski, B. J. & Geib, S. M. Rapid viral symbiogenesis via changes in parasitoid wasp genome architecture. Mol. Biol. Evol. 35, 2463–2474 (2018).
Di Giovanni, D. et al. A behavior-manipulating virus relative as a source of adaptive genes for Drosophila parasitoids. Mol. Biol. Evol. 37, 2791–2807 (2020).
Gitau, C. W., Gundersen-Rindal, D., Pedroni, M., Mbugi, P. J. & Dupas, S. Differential expression of the CrV1 haemocyte inactivation-associated polydnavirus gene in the African maize stem borer Busseola fusca (Fuller) parasitized by two biotypes of the endoparasitoid Cotesia sesamiae (Cameron). J. Insect Physiol. 53, 676–684 (2007).
Veiga, A. C. P., Vacari, A. M., Volpe, H. X. L., de Laurentis, V. L. & De Bortoli, S. A. Quality control of Cotesia flavipes (Cameron) (Hymenoptera: Braconidae) from different Brazilian bio-factories. Biocont. Sci. Technol. 23, 665–673 (2013).
Geervliet, J. B. F., Vet, L. E. M. & Dicke, M. Volatiles from damaged plants as major cues in long‐range host‐searching by the specialist parasitoid Cotesia rubecula. Entomol. Exp. et. Applicata 73, 289–297 (1994).
Smid, H. M. et al. Species-specific acquisition and consolidation of long-term memory in parasitic wasps. Proc. Biol. Sci. 274, 1539–1546 (2007).
Alberti, A. et al. Viral to metazoan marine plankton nucleotide sequences from the Tara Oceans expedition. Sci. Data 4, 170093 (2017).
Margulies, M. et al. Genome sequencing in microfabricated high-density picolitre reactors. Nature 437, 376–380 (2005).
Aury, J. M. et al. High quality draft sequences for prokaryotic genomes using a mix of new sequencing technologies. BMC Genomics 9, 603 (2008).
Luo, R. et al. SOAPdenovo2: an empirically improved memory-efficient short-read de novo assembler. Gigascience 1, 18 (2012).
Marbouty, M. et al. Metagenomic chromosome conformation capture (meta3C) unveils the diversity of chromosome organization in microorganisms. Elife 3, e03318 (2014).
Langmead, B. & Salzberg, S. L. Fast gapped-read alignment with Bowtie 2. Nat. Methods 9, 357–359 (2012).
Baudry, L. et al. instaGRAAL: chromosome-level quality scaffolding of genomes using a proximity ligation-based scaffolder. Genome Biol. 21, 148 (2020).
Mikheenko, A., Prjibelski, A., Saveliev, V., Antipov, D. & Gurevich, A. Versatile genome assembly evaluation with QUAST-LG. Bioinformatics 34, i142–i150 (2018).
Waterhouse, R. M. et al. BUSCO Applications from quality assessments to gene prediction and phylogenomics. Mol. Biol. Evol. 35, 543–548 (2018).
Flutre, T., Duprat, E., Feuillet, C. & Quesneville, H. Considering transposable element diversification in de novo annotation approaches. PLoS ONE 6, e16526 (2011).
Korf, I. Gene finding in novel genomes. BMC Bioinforma. 5, 59 (2004).
Cantarel, B. L. et al. MAKER: an easy-to-use annotation pipeline designed for emerging model organism genomes. Genome Res. 18, 188–196 (2008).
Camacho, C. et al. BLAST+: architecture and applications. BMC Bioinforma. 10, 421 (2009).
Jones, P. et al. InterProScan 5: genome-scale protein function classification. Bioinformatics 30, 1236–1240 (2014).
Conesa, A. et al. Blast2GO: a universal tool for annotation, visualization and analysis in functional genomics research. Bioinformatics 21, 3674–3676 (2005).
Dunn, N. A. et al. Apollo: Democratizing genome annotation. PLoS Comput. Biol. 15, e1006790 (2019).
Buchfink, B., Xie, C. & Huson, D. H. Fast and sensitive protein alignment using DIAMOND. Nat. Methods 12, 59–60 (2015).
Kumar, S., Jones, M., Koutsovoulos, G., Clarke, M. & Blaxter, M. Blobology: exploring raw genome data for contaminants, symbionts and parasites using taxon-annotated GC-coverage plots. Front. Genet. 4, 237 (2013).
Emms, D. M. & Kelly, S. OrthoFinder: solving fundamental biases in whole genome comparisons dramatically improves orthogroup inference accuracy. Genome Biol. 16, 157 (2015).
Katoh, K., Misawa, K., Kuma, K. & Miyata, T. MAFFT: a novel method for rapid multiple sequence alignment based on fast Fourier transform. Nucleic Acids Res. 30, 3059–3066 (2002).
Guindon, S. & Gascuel, O. A simple, fast, and accurate algorithm to estimate large phylogenies by maximum likelihood. Syst. Biol. 52, 696–704 (2003).
Darriba, D., Taboada, G. L., Doallo, R. & Posada, D. jModelTest 2: more models, new heuristics and parallel computing. Nat. Methods 9, 772 (2012).
Zhou, X. et al. Chemoreceptor Evolution in Hymenoptera and Its Implications for the Evolution of Eusociality. Genome Biol. Evol. 7, 2407–2416 (2015).
Robertson, H. M., Gadau, J. & Wanner, K. W. The insect chemoreceptor superfamily of the parasitoid jewel wasp Nasonia vitripennis. Insect Mol. Biol. 19, 121–136 (2010).
Robertson, H. M. & Wanner, K. W. The chemoreceptor superfamily in the honey bee, Apis mellifera: expansion of the odorant, but not gustatory, receptor family. Genome Res. 16, 1395–1403 (2006).
Chen, K., Durand, D. & Farach-Colton, M. NOTUNG: a program for dating gene duplications and optimizing gene family trees. J. Comput. Biol. 7, 429–447 (2000).
Stolzer, M. et al. Inferring duplications, losses, transfers and incomplete lineage sorting with nonbinary species trees. Bioinformatics 28, i409–i415 (2012).
Ranwez, V., Harispe, S., Delsuc, F. & Douzery, E. J. MACSE: Multiple alignment of coding sequences accounting for frameshifts and stop codons. PLoS ONE 6, e22594 (2011).
Yang, Z. PAML 4: phylogenetic analysis by maximum likelihood. Mol. Biol. Evol. 24, 1586–1591 (2007).
Kim, D. et al. TopHat2: accurate alignment of transcriptomes in the presence of insertions, deletions and gene fusions. Genome Biol. 14, R36 (2013).
Liao, Y., Smyth, G. K. & Shi, W. The Subread aligner: fast, accurate and scalable read mapping by seed-and-vote. Nucleic Acids Res. 41, e108 (2013).
Robinson, M. D., McCarthy, D. J. & Smyth, G. K. edgeR: a Bioconductor package for differential expression analysis of digital gene expression data. Bioinformatics 26, 139–140 (2010).
Robinson, M. D. & Oshlack, A. A scaling normalization method for differential expression analysis of RNA-seq data. Genome Biol. 11, R25 (2010).
Lund, S. P., Nettleton, D., McCarthy, D. J. & Smyth, G. K. Detecting differential expression in RNA-sequence data using quasi-likelihood with shrunken dispersion estimates. Stat. Appl. Genet. Mol. Biol. 11, 23104842 (2012).
Benjamini, Y. & Hochberg, Y. Controlling the false discovery rate: a practical and powerful approach to multiple testing. J. R. Stat. Soc. B 57, 289–300 (1995).
Gauthier, J. Custom scripts for Cotesia genomes analyses. Zenodo https://doi.org/10.5281/zenodo.4116412 (2020).
We thank Paul André Catalayud for providing the pictures of C. sesamiae and C. flavipes Germain Chevignon for the pictures of C. congregata nymphal stages and Juline Herbinière for TEM images of C. congregata ovaries. We thank the ADALEP (Adaptation of Lepidoptera) network for the involvement of its members and access to bioinformatic facilities for genome annotation. C. sesamiae individuals used in this study originated from the icipe, under the juridical framework of a Material Transfer Agreement signed between IRD, icipe and CNRS (CNRS 072057/IRD 302227/00). The authors thank Bruno Le Ru, Gerphas Ogola, and Julius Obonyo, which made the insects accessible for the study. C. congregata, C. sesamiae, C. flavipes genomes sequencing were funded by French National Research Agency ANR (ABC Papogen project ANR-12-ADAP-0001 and CoteBio ANR17-CE32-0015-02 to L. Kaiser). C. rubecula, C. glomerata, C. vestalis genomes sequencing were funded by NWO EcoGenomics grant 844.10.002 to L.E.M. Vet, NWO VENI grant 863.07.010 and Enabling Technology Platform Hotel grant to L.E.M. Vet. HiC approach was funded by ERC project 260822 to R. Koszul. C. congregata transcriptomic analysis was funded by APEGE project (CNRS-INEE) to J.-M. Drezen. J. Gauthier thesis was funded by ANR and Region Center-Val de Loire. Collaboration between French and Netherland laboratories was funded by French ministry of foreign affairs and “Nuffic” (“VanGogh” Project to J.-M. Drezen and L.E.M. Vet).
The authors declare no competing interests.
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Gauthier, J., Boulain, H., van Vugt, J.J.F.A. et al. Chromosomal scale assembly of parasitic wasp genome reveals symbiotic virus colonization. Commun Biol 4, 104 (2021). https://doi.org/10.1038/s42003-020-01623-8