Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

Candidatus Sodalis melophagi sp. nov.: Phylogenetically Independent Comparative Model to the Tsetse Fly Symbiont Sodalis glossinidius

  • Tomáš Chrudimský ,

    Affiliation Faculty of Science, University of South Bohemia, České Budějovice, Czech Republic

  • Filip Husník,

    Affiliations Faculty of Science, University of South Bohemia, České Budějovice, Czech Republic, Institute of Parasitology, Biology Centre, Academy of Sciences of the Czech Republic, České Budějovice, Czech Republic

  • Eva Nováková,

    Affiliations Faculty of Science, University of South Bohemia, České Budějovice, Czech Republic, Institute of Parasitology, Biology Centre, Academy of Sciences of the Czech Republic, České Budějovice, Czech Republic

  • Václav Hypša

    Affiliations Faculty of Science, University of South Bohemia, České Budějovice, Czech Republic, Institute of Parasitology, Biology Centre, Academy of Sciences of the Czech Republic, České Budějovice, Czech Republic

Candidatus Sodalis melophagi sp. nov.: Phylogenetically Independent Comparative Model to the Tsetse Fly Symbiont Sodalis glossinidius

  • Tomáš Chrudimský, 
  • Filip Husník, 
  • Eva Nováková, 
  • Václav Hypša


Bacteria of the genus Sodalis live in symbiosis with various groups of insects. The best known member of this group, a secondary symbiont of tsetse flies Sodalis glossinidius, has become one of the most important models in investigating establishment and evolution of insect-bacteria symbiosis. It represents a bacterium in the early/intermediate state of the transition towards symbiosis, which allows for exploring such interesting topics as: usage of secretory systems for entering the host cell, tempo of the genome modification, and metabolic interaction with a coexisting primary symbiont. In this study, we describe a new Sodalis species which could provide a useful comparative model to the tsetse symbiont. It lives in association with Melophagus ovinus, an insect related to tsetse flies, and resembles S. glossinidius in several important traits. Similar to S. glossinidius, it cohabits the host with another symbiotic bacterium, the bacteriome-harbored primary symbiont of the genus Arsenophonus. As a typical secondary symbiont, Candidatus Sodalis melophagi infects various host tissues, including bacteriome. We provide basic morphological and molecular characteristics of the symbiont and show that these traits also correspond to the early/intermediate state of the evolution towards symbiosis. Particularly, we demonstrate the ability of the bacterium to live in insect cell culture as well as in cell-free medium. We also provide basic characteristics of type three secretion system and using three reference sequences (16 S rDNA, groEL and spaPQR region) we show that the bacterium branched within the genus Sodalis, but originated independently of the two previously described symbionts of hippoboscoids. We propose the name Candidatus Sodalis melophagi for this new bacterium.


The genus Sodalis belongs to the symbiotic bacterial lineages that adopted several different types of symbiosis with their hosts, ranging from facultative commensals to obligate mutualists [1], [2]. Sodalis and closely related bacteria were described from a broad spectrum of insect hosts including tsetse flies [3], weevils [4][7], chewing lice [8], hippoboscid louse flies [9], ants [10], scale insects [11], aphids [12], stinkbugs [13], [14], and cerambycid beetles [15]. Also, some “secondary” symbionts of psyllids and mealybugs cluster with the Sodalis clade [16], [17]. Within symbiotic Enterobacteriaceae, diversity of the Sodalis clade is comparable only with the genus Arsenophonus [18].

The first described, best known and most frequently investigated member of the genus is S. glossinidius, S-symbiont of tsetse flies [3]. Its significance for the host is still not clear, but a possible influence on the host longevity and resistance to trypanosomes has previously been suggested [19]. Several molecular analyses and genetic experiments made S. glossinidius an important model for investigating evolution and biology of symbiotic bacteria [20][22]. It has been employed in research of various biological traits, such as the structure and role of secretion systems [21], the function of the iron acquisition system [23] or the usage of the quorum sensing system [24]. Moreover, S. glossinidius proved to be among the few symbionts that could be maintained in in vitro culture in insect cells as well as in the cell-free media [3], [25]. This feature has been attributed to the initial or intermediate state of the S. glossinidius shift towards symbiosis. One of the most frequently discussed topics in this respect is the state and function of the type three secretion system (TTSS) in this bacterium. Three different copies of the TTSS (SSR-1, SSR-2 and SSR-3) has been detected in S. glossinidius [26], [27] and a possible role of the SSR-2 in invading host cells has been proposed [21].

Within the host, S. glossinidius constitutes part of a complex bacterial community which also contains P-symbiont Wigglesworthia glossinidia [28] and alphaproteobacterium Wolbachia [29], [30]. Recent investigations show that the whole community may be even richer and contain an array of other bacteria [31]. Such complex host-symbiont systems provide a unique opportunity for comparing genomes in different states/modes of symbiosis and studying processes of their metabolic complementation [32], [33]. For the Sodalis-Wigglesworthia-Glossina association, complete genomes of both bacteria have been sequenced and annotated [26], [34]. Even though each of the sequenced genomes came from different host species, an interaction between Sodalis and Wigglesworthia via thiamine synthesis could be detected by their comparison [27] and this view was further corroborated by an experimental approach [35] and sequencing of Wigglesworthia lineage from Glossina morsitans [36].

An establishment of a more complete picture of Sodalis genome evolution will require complete genome sequences for a more diverse array of Sodalis isolates, and of similar complex systems involving this bacterium. Although tsetse flies are the most important blood feeding brachycerans, there are several related groups of dipterans that display many similar features such as the feeding strategy, vivipary and transmission of trypanosomes.

A member of the genus Sodalis, phylogenetically independent on the tsetse symbiont, has already been described from hippoboscoid species Craterina melbae [9]. Here, we characterize a new member of the Sodalis lineage, inhabiting gut and other tissues of another hippoboscoid, Melophagus ovinus. The presence of several symbiotic bacteria in this species has long been known. According to morphological investigations of several researchers summarized by Paul Buchner [37], Melophagus ovinus contains symbiotic bacteria within enlarged epithelial cells of a specialized section of the midgut (bacteriome). This P-symbiont was recently characterized by molecular techniques as a member of Arsenophonus clade and is likely to play a role resembling that of Wigglesworthia in tsetse flies (Nováková et al., in prep). In addition, some of the authors recognized two other bacteria in the sheep keds. The first is Bartonella melophagi (originally described as Rickettsia melophagi and Wolbachia melophagi), which is localized extracellularly along microvilli of the midgut. The second type of bacterium described in Paul Buchner’s work resembles Candidatus Sodalis melophagi as presented in this study: “In the low zones of the midgut epithelium…, there are additional delicate bacteria, sometimes forming rather long filaments, which also must not be confused with the symbionts.” The whole system thus remarkably resembles the Wigglesworthia-Sodalis association in tsetse flies and can provide important data for a comparative study. In this study, we present a basic molecular and morphological characterization of the new Sodalis linage and overview the composition of its TTSS. We suggest the new name Candidatus Sodalis melophagi for this bacterium and extend the available Sodalis spectrum with three additional samples which allow for more precise phylogenetic characterization.


Sequence Data

Sequences obtained by PCR for the investigated samples and their accession numbers are summarized in Table S1. The 16 S rDNA sequence from Candidatus Sodalis melophagi sp. nov. displayed 98.48% similarity to 16 S rDNA of S. glossinidius. Illumina assemblies produced preliminary draft sequences from which only selected gene regions were used here for the formal description and basic phylogenetic characterization. These regions, including all TTSS genes (Table S1) and groEL chaperonin, were of a high quality and did not contain any SNPs. In order to avoid assembly artifacts affecting the sequence accuracy of highly similar paralogous regions, a partial sequence for 16 S rRNA gene was obtained through Sanger sequencing as described above and was used for inferring phylogeny. Sanger sequenced groEL partial sequence was identical to the sequence acquired from Illumina data and we therefore used the full length groEL for phylogenetic reconstruction.

Type Three Secretion System (TTSS)

Candidatus Sodalis melophagi possesses only SSR-2 and SSR-3 copies of the TTSS in its genome, while SSR-1 is completely missing. Extensive BLASTX searches did not produce any significant hits for S. glossinidius SSR-1 either in Illumina contigs or raw reads. The gene order and content of SSR-2 and SSR-3 of Candidatus Sodalis melophagi is very similar, but not identical to that in S. glossinidius (Figure 1). The SSR-2 sequence comprises 11 protein coding genes: orgAbA, prgKIH, spaSQPO, invF and hilA; and 5 pseudogenes: prgJ, sicA, spaR and invAG. In comparison with S. glossinidius, it lacks 4 genes: invB, invC and spaLMN. The SSR-3 comprises 29 protein coding genes: ssrAB, ssaBCDEGHIJKLMNOPQRSTUV, sseABCDE, sscB, a protein similar to locus SG1296 of S. glossinidius, and a single pseudogene: sscA. Sequences of Candidatus Sodalis melophagi TTSS genes were deposited in GenBank as a part of two annotated contigs for each of the islands (Table S1).

Figure 1. Composition of SSR-2 and SSR-3 copies of Candidatus Sodalis melophagi TTSS.

Ψ – putative pseudogene (see Material and Methods).

Phylogenetic Analyses

The lengths of individual matrices and numbers of variable positions are summarized in Table S2. All phylogenetic trees clearly indicate that the novel bacterium belongs to the genus Sodalis (Figures 2, 3, 4, Figure S1, Figure S2). In the trees derived from 16 S rRNA gene sequence data and amino acid sequence of groEL, Candidatus Sodalis melophagi clusters within a large polytomy and its precise position within the genus is thus uncertain (Figures 23A, Figure S1, Figure S2). However, even this unresolved topology excludes its relationship to any of the two other hippoboscoid-derived Sodalis members. This conclusion is further supported by the nucleotide matrix for groEL (Figure 3B) with a reduced sampling and the spaPQR concatenate (Figure 4). Although the exact topology slightly varies with the methods and parameters of the analysis, the three hippoboscoid lineages always form a polyphyletic/paraphyletic assemblage.

Figure 2. 16 S rDNA tree derived by BI analysis in MrBayes.

Posterior probabilities are indicated by the numbers at the nodes. New Sodalis lineages added in this study are printed in red.

Figure 3. Phylogenetic trees derived from groEL matrices by BI in MrBayes.

New Sodalis lineages added in this study are printed in red. A: The tree inferred from aminoacid matrix. Posterior probabilities are indicated by the numbers at the nodes. B: The tree inferred from nucleotide matrix restricted taxonomically to the Sodalis branch. The numbers at the nodes show the posterior probabilities and bootstrap values from the identical topology obtained by ML in PhyML.

Figure 4. Phylogenetic tree derived from spaPQR region by BI in MrBayes.

The numbers at the nodes show the posterior probabilites and bootstrap values from the identical topology obtained by ML in PhyML. New Sodalis lineages added in this study are printed in red.

In vitro Culture

Bacterial colonies were clearly visible after 8 days of cultivation. Colonies were white, raised, and circular with entire edges. Their size was irregular ranging from 0.5 to 1 mm. The variable size of the colonies was almost certainly not due to new mutations, since subculturing on fresh plates yielded the same variability for each individual colony. The irregular colony morphology was described also in case of a type strain M1T of the Sodalis glossinidius [3] and is probably population dependent as is the case in other microaerophilic bacteria [38].

The type strain CZT was established by isolation of a single bacterial colony and was used for C6/36 cells infection. In the C6/36 cell culture, bacteria were predominantly attached to cell surface or free in the medium, but they were also observed inside the cells. Genomic DNA purified from bacterial colonies of Candidatus Sodalis melophagi CZT was used as a template for Illumina mate pair sequencing.


Under electron microscopy, Sodalis cells within the host tissue corresponded well to their light microscope characteristics (Figure 5A). They appeared as rods reaching from approx. 1 to 4 μm, depending on the angle of the section, and were located mainly at the periphery of the bacteriome, sometimes in close association with the P-symbionts (Figures 5B,C).

Figure 5. Morphology and ultrastructure of Candidatus Sodalis melophagi.

A: In vitro cell culture in Nomarski contrast. B, C: Cells of Candidatus Sodalis melophagi in bacteriome. Black arrows – cells of Candidatus Sodalis melophagi, white arrows – cells of the primary endosymbiont of the genus Arsenophonus.

Description of Candidatus Sodalis Melophagi sp. nov

Candidatus Sodalis melophagi (me.lo.phag.í; melophagi of the genus Melophagus).

Candidatus Sodalis melophagi is a Gram-negative bacterium isolated from the sheep ked Melophagus ovinus. The bacteria were detected in heamolymph and bacteriome. The cells are rod-shaped non-motile and non-spore forming under laboratory conditions. The average length is 1.9 μm, however, bacteria ranging from 0.6 to 5 μm in length were observed. The bacteria grow intracelullarly and extracellularly in presence of Aedes albopictus cell line C6/36 under aerobic conditions. They can also be cultivated axenically both in liquid and solid media containing enzymatically digested proteins as a source of nitrogen, with the addition of blood under the microaerophilic atmosphere (5% O2 balanced with carbon dioxide) at 27°C.


Remarkably, the main biological traits of Candidatus Sodalis melophagi and its relation to the host resemble those of Sodalis glossinidus in tsetse flies. In both cases the hosts are exclusively blood feeding organisms reproducing by vivipary and their Sodalis plays a role of an “accessory” symbiont accompanying phylogenetically distant P-symbiont (Wigglesworthia in tsetse flies and Arsenophonus in Melophagus). This status of Candidatus Sodalis melophagi is strongly indicated by phylogenetic characteristics as well as location and morphology revealed by electron microscopy. Similar to S. glossinidius, the rod-shaped cells of Candidatus Sodalis melophagi are not restricted to the bacteriocytes but they infect various non-specialized cells and can be cultivated from haemolyph. It is therefore interesting to note that according to phylogenetic analyses its symbiosis with the host originated independently of the S. glossinidius as well as of the third hipoboscoid lineage, the symbiont of Craterina melbae. Although exact position of Candidatus Sodalis melophagi within the Sodalis clade varies with method and taxon sampling, it never clusters with any of the two other hippoboscoid-derived lineages. Within the Sodalis clade, such host-symbiont incongruence is not unique to the hippoboscoid-derived lineages. It is also expressed by the distribution of several other samples, particularly those from coleopteran and homopteran hosts (Figure 2, Figure S1) and clearly demonstrates the capability of Sodalis to spread by horizontal transfers. In contrast, the close relationships of the two new 16 S rDNA sequences obtained from Ornithomya with the Sodalis previously described from Craterina melbae suggests that these two hippoboscoid genera may share the same symbiotic lineage inherited from their common ancestor. However, the sampling of Sodalis lineages available from other insect groups is highly incomplete. In addition, the position of some sequences, such as Sodalis from Sitophilus rugicollis is affected by long-branch attraction due to the high AT content; instability of this lineage has been found in previous analyses [9]. Thus, although we extended the sampling with additional three sequences, any interpretations of the modes and mechanism of Sodalis transmission can under the current circumstances be only working hypotheses rather than serious conclusions based on the data.

While the draft genomic data of Candidatus Sodalis melophagi is currently under investigation, we preliminarily analyzed the composition and structure of the TTSS. Significance of this system in symbiosis evolution has previously been suggested [39] and investigated in several symbiotic lineages [21], [40][43]. These genes are also among the few sequences that are currently available and can be compared between different Sodalis taxa. In S. glossinidius, experimental work indicated that TTSS of SPI1 type from Salmonella (later designated as SSR-2) is essential for entering the host cell. Presence and apparent functionality of this system was subsequently confirmed in another Sodalis, the primary endosymbiont of Sitophilus zeamais (SZPE) [42]. However, further studies revealed another two copies of TTSS in S. glossinidius genome, SSR-1 closely related to the Ysa system of Yersinia, and SSR-3 related to Salmonella SPI2 [26], [27], [40]. The secretion systems in Candidatus Sodalis melophagi show clear similarity to S. glossinidius genes but the whole machinery is much less complex; SSR-1 is completely missing and SSR-2 is highly eroded. However, the form corresponding to the SSR-3 is complete and possibly functional. Its structure and gene content is highly similar to that in S. glossinidius, except for a pseudogenized state of sscA, encoding a putative chaperone of secreted protein SseC [44].

The differences between TTSS in S. glossinidius and Candidatus Sodalis melophagi pose an interesting question about the origin, role and significance of TTSS and its different copies in the genus Sodalis. As the two compared lineages, Candidatus Sodalis melophagi and S. glossinidius are not closely related and the whole Sodalis tree is currently undersampled, it is impossible to hypothesize whether SSR-1 was lost in the former one or acquired by the latter one after diversification of their ancestor. The significance of TTSS in the two lineages is even more difficult to assess. In Candidatus Sodalis melophagi, the SSR-3 alone or possibly in synergy with the retained functional genes of SSR-2, seems to be sufficient for maintenance of the intracellular lifestyle. This view, however, is based solely on the observed presence/absence of the genes and their comparison to the experimental results from S. glossinidius [21]. It should be taken into account that other related systems, such as flagellar export apparatus, can participate in the host cell invasion. Despite the knockout experiments, the situation is similarly unclear in S. glossinidius where the presence of SSR-3 has not been known at the time of the experimental work and its significance could not be investigated. From the genomic point of view, S. glossinidius has so far been the only member of the genus for which a detailed characterization of the genome and some metabolic capabilities is available. The quality of Candidatus Sodalis melophagi paired-end data retrieved from the bacteriome sequencing and additional mate pair data recently obtained from the pure culture suggest that a draft genome of this symbiont could be established and used for further comparisons. Such analysis, comparing reduction, structure, and possible adaptive changes of independent but closely related bacteria from two hosts with similar but unique biology will provide important insight into the symbiogenetic processes. In respect to the future work, it may help to discriminate between the random and symbiosis-associated modifications and indicate candidate genes for a more detailed investigation.

Materials and Methods

Ethic Statement

All field studies did not involve protected or endangered organisms. They were not performed on privately-owned or protected locations and were performed according to the law of the Czech Republic.

Insect Samples, DNA Extraction, Sequencing and Data Assembly

Adults of Melophagus ovinus were obtained commercially from a licensed family sheep farm at Krásetín, Czech Republic. A midgut region with the bacteriome was dissected into the phosphate buffered saline (PBS) and total genomic DNA was extracted from each single adult by QIAamp DNA Micro Kit (Qiagen). DNA concentration was determined using NanoDrop2000 (Thermo Scientific) and its quality was assessed in 2% agarose gel using standard electrophoresis. PCR was carried out as described previously [18] with bacterial primers for 16 S rDNA and groEL (Table S3). The same procedure was followed for three additional samples. Two of them were Sodalis bacteria from other insect hosts, Ornithomya avicularia (Diptera, Hippoboscidae) and Rhampus pulicarius (Coleoptera, Curculionidae), and the third was Biostraticola tofi strain BF36T, a free-living bacterium supposedly closely related to Sodalis [45]. Laboratory culture of B. tofi was obtained from the DSMZ microorganism collection (Germany), R. pulicarius was collected near České Budějovice (Czech Republic); according to the law of the Czech Republic, no permits are required for collection of this organism. Samples of O. avicularia were provided by Department of Zoology (University of South Bohemia); the collections were done during the ornithological research performed in accordance with the law of the Czech Republic.

We used 3 μg of genomic DNA isolated from M. ovinus bacteriome as a template for an Illumina paired-end library with an insert size of 300 bp. Library construction and sequencing on one lane in a 100 bp run was carried out at Keck Microarray Resource, West Haven CT, USA. Reads obtained underwent adaptor and quality trimming, and were further processed using two different approaches. First, the reads with significant BLASTN [46] hit to Sodalis glossinidius genome sequence (NC_007712) were filtered and the retrieved subset was assembled using CLC Genomic Workbench (CLC bio A/S) with parameters set to the following values: similarity 0.9, length fraction 0.9, costs for deletion/insertion/mismatch 3. Second, de-novo assembly of all the processed reads into contigs was done on CLC Genomic Workbench (CLC bio A/S) under the same parameter setting. Contigs from this assembly were binned based on their average coverage and BlastX [46] hits against available bacterial genomes. Since some of the sequences were used in this study for phylogenetic reconstruction, we checked the accuracy of the Illumina-derived sequences by an independent Sanger sequencing of the groEL gene.

Type Three Secretion System (TTSS) Annotation

Contigs spanning corresponding genes to TTSS islands from Sodalis glossinidius were retrieved based on the Blast X [46] results from both assemblies. In order to obtain a single contig for each of the TTSS islands, gaps were closed using targeted Sanger sequencing (Table S3). Mapped sequences were checked for presence of single nucleotide polymorphisms (SNPs). ORF prediction was done using CLC Genomic Workbench (CLC bio A/S) with the minimum length set to 30 AA. Gene annotation based on similarity confirmed by BLAST searches was performed manually in the same software. All genes that contained frame shift mutation or stop mutations were tentatively classified as pseudogenes. The hilA previously classified as pseudogene [26], [27] was annotated as functional based on recent experimental work [47].

Phylogenetic Analyses

We used three different regions for the phylogenetic reconstruction, 16 S rDNA, groEL and the TTSS region consisting of the spaP-spaQ-spaR genes (, S5, S6). The groEL amino acid dataset was aligned using ClustalW algorithm in BioEdit with default parameters [48] and all ambiguously aligned sites were removed from the further analyses. To gain more precise phylogenetic resolution within the Sodalis branch, we narrowed the taxon sampling and prepared an additional matrix using nucleotide sequences for the groEL gene. The matrix was aligned as described above and edited manually. The 16 S rDNA and the spaPQR dataset were aligned in the Mafft program [49], using the E-INS-i strategy with default parameters and manually edited in BioEdit [48]. For 16 S rDNA, the ambiguously aligned positions were eliminated in Gblocks [50].

Two approaches were used to infer phylogenetic trees, maximum likelihood (ML) and Bayesian inference (BI). For ML we used PhyML v3.0 [51], [52] with the SPR search algorithm. BI was performed in MrBayes 3.1.2 [53], [54] with five million generations and tree sampling every 100 generations. AWTY [55] was used to check the MCMC convergence and determine burn-in. Evolutionary substitution models for proteins and DNA were selected by ProtTest 2.4 [56] and for DNA by jModelTest 0.1.1 [57], respectively. For DNA sequences, the General Time Reversible (GTR) model was used with an estimated proportion of invariable sites (I) and heterogeneity of evolutionary rates modeled by the eight substitution rate categories of the gamma (Γ) distribution and the gamma shape parameter (alpha) estimated from the data. LG+I+Γ was determined as the best fitting model for the amino acid groEL dataset, and it was used for the ML analyses. Since this model is not implemented in MrBayes, we replaced it with WAG+I+Γ for the BI analysis. JTT+I+Γ model was used for the spaPQR concatenate in both BI and ML analyses.

Cultivation of Candidatus Sodalis Melophagi sp. nov

The insects were surface sterilized using 96% ethanol and heamolymph was collected into a 1.5 ml eppendorf tube containing 500 μl of Mitsuhashi-Maramorosch (MM) medium [58] with 20% heat inactivated foetal bovine serum (FBS). The tube was incubated overnight at 27°C without shaking, a slightly modified protocol of Matthew et al. [25] was followed. Liquid culture was plated onto 10% sheep blood MMI plates solidified by 1% agar. The medium was supplemented with 100 μg/ml Polymyxin B and 10 mg/ml Amphotericin B to prevent contamination by Gram-negative non-symbiotic bacteria [59] and fungi. The plates were incubated at 27°C in a microaerobic atmosphere generated by the Campygen pack system (Oxoid) producing 5% of oxygen balanced with carbon dioxide. Bacteria were further inoculated into flasks containing C6/36 mosquito cells [60] (LGC Standards, Czech Republic) in MM medium with 20% heat inactivated FBS.


A three day old liquid culture of C6/36 cells infected with Candidatus Sodalis melophagi was used for microscopic examination. Cells were harvested and fixed in 4% formaldehyde in PBS and observed under the BX53 microscope (Olympus) using Nomarski contrast. For electron microscopy, the midgut region containing bacteriome was dissected directly into a 2.5% glutaraldehyde in 0.1 M phosphate buffer and prefixed at 4°C overnight. The tissue was then postfixed at 4°C for 60 min with 2% osmium tetroxide in phosphate buffer. After dehydration through ethanol series, the samples were embedded in Spurr resin. Ultrathin sections were stained with uranyl acetate and lead citrate and examined in transmission electron microscope JEOL JEM-1010.

Supporting Information

Figure S1.

16 S rDNA tree derived by ML method in PhyML. Bootstrap values are indicated by the numbers at the nodes. New Sodalis lineages added in this study are printed in red. Values under 50 are not shown.



Figure S2.

Phylogenetic trees derived from groEL aminoacid matrix under ML in PhyML. Bootstrap values are indicated by the numbers at the nodes. New Sodalis lineages added in this study are printed in red. Values under 50 are not shown.



Table S1.

List of sequences acquired in this study.



Table S2.

Characteristics of particular datasets.



Table S3.

List of primers used in this study.



Table S4.

List of 16 S rDNA sequences used for phylogenetic inference.



Table S5.

List of groEL sequences used for phylogenetic inference.



Table S6.

List of spaPQR sequences used for phylogenetic inference.




We are grateful to Nancy A. Moran and Keck Microarray Resource for technical assistance with the genome sequencing.

Author Contributions

Wrote the paper: TC FH EN VH. Designed the study: EN VH. Established in vitro culture: TC FH. Generated and assembled the genomic data: EN. Performed the light and electron microscopy characterization: TC FH VH. Performed phylogenetic analyses: TC FH. Annotated and analyzed the TTSS sequences: TC.


  1. 1. Snyder AK, McMillen CM, Wallenhorst P, Rio RV (2011) The phylogeny of Sodalis-like symbionts as reconstructed using surface-encoding loci. FEMS Microbiol Lett 317: 143–151.
  2. 2. Heddi A, Charles H, Khatchadourian C, Bonnot G, Nardon P (1998) Molecular characterization of the principal symbiotic bacteria of the weevil Sitophilus oryzae: a peculiar G + C content of an endocytobiotic DNA. J Mol Evol 47: 52–61.
  3. 3. Dale C, Maudlin I (1999) Sodalis gen. nov. and Sodalis glossinidius sp. nov., a microaerophilic secondary endosymbiont of the tsetse fly Glossina morsitans morsitans. Int J Syst Bacteriol 49 Pt 1: 267–275.
  4. 4. Toju H, Hosokawa T, Koga R, Nikoh N, Meng XY, et al. (2010) “Candidatus Curculioniphilus buchneri,” a novel clade of bacterial endocellular symbionts from weevils of the genus Curculio. Appl Environ Microbiol 76: 275–282.
  5. 5. Toju H, Fukatsu T (2011) Diversity and infection prevalence of endosymbionts in natural populations of the chestnut weevil: relevance of local climate and host plants. Mol Ecol 20: 853–868.
  6. 6. Conord C, Despres L, Vallier A, Balmand S, Miquel C, et al. (2008) Long-term evolutionary stability of bacterial endosymbiosis in curculionoidea: additional evidence of symbiont replacement in the dryophthoridae family. Mol Biol Evol 25: 859–868.
  7. 7. Campbell BC, Bragg TS, Turner CE (1992) Phylogeny of symbiotic bacteria of four weevilspecies (coleoptera: curculionidae) based on analysis of 16 S ribosomal DNA. Insect Biochem Mol Biol 22: 415–421.
  8. 8. Fukatsu T, Koga R, Smith WA, Tanaka K, Nikoh N, et al. (2007) Bacterial endosymbiont of the slender pigeon louse, Columbicola columbae, allied to endosymbionts of grain weevils and tsetse flies. Appl Environ Microbiol 73: 6660–6668.
  9. 9. Nováková E, Hypša V (2007) A new Sodalis lineage from bloodsucking fly Craterina melbae (Diptera, Hippoboscoidea) originated independently of the tsetse flies symbiont Sodalis glossinidius. FEMS Microbiol Lett 269: 131–135.
  10. 10. Sameshima S, Hasegawa E, Kitade O, Minaka N, Matsumoto T (1999) Phylogenetic comparison of endosymbionts with their host ants based on molecular evidence. Zoolog Sci 16: 993–1000.
  11. 11. Gruwell ME, Hardy NB, Gullan PJ, Dittmar K (2010) Evolutionary relationships among primary endosymbionts of the mealybug subfamily phenacoccinae (hemiptera: Coccoidea: Pseudococcidae). Appl Environ Microbiol 76: 7521–7525.
  12. 12. Burke GR, Normark BB, Favret C, Moran NA (2009) Evolution and diversity of facultative symbionts from the aphid subfamily Lachninae. Appl Environ Microbiol 75: 5328–5335.
  13. 13. Kaiwa N, Hosokawa T, Kikuchi Y, Nikoh N, Meng XY, et al. (2010) Primary gut symbiont and secondary, Sodalis-allied symbiont of the Scutellerid stinkbug Cantao ocellatus. Appl Environ Microbiol 76: 3486–3494.
  14. 14. Kaiwa N, Hosokawa T, Kikuchi Y, Nikoh N, Meng XY, et al. (2011) Bacterial symbionts of the giant jewel stinkbug Eucorysses grandis (Hemiptera: Scutelleridae). Zoolog Sci 28: 169–174.
  15. 15. Grünwald S, Pilhofer M, Höll W (2010) Microbial associations in gut systems of wood- and bark-inhabiting longhorned beetles (Coleoptera: Cerambycidae). Syst Appl Microbiol 33: 25–34.
  16. 16. Thao ML, Clark MA, Baumann L, Brennan EB, Moran NA, et al. (2000) Secondary endosymbionts of psyllids have been acquired multiple times. Curr Microbiol 41: 300–304.
  17. 17. Thao ML, Gullan PJ, Baumann P (2002) Secondary (γ-Proteobacteria) endosymbionts infect the primary (β-Proteobacteria) endosymbionts of mealybugs multiple times and coevolve with their hosts. Appl Environ Microbiol 68: 3190–3197.
  18. 18. Nováková E, Hypša V, Moran NA (2009) Arsenophonus, an emerging clade of intracellular symbionts with a broad host distribution. BMC Microbiol 9: 143.
  19. 19. Dale C, Welburn SC (2001) The endosymbionts of tsetse flies: manipulating host-parasite interactions. Int J Parasitol 31: 628–631.
  20. 20. Pontes MH, Dale C (2011) Lambda red-mediated genetic modification of the insect endosymbiont Sodalis glossinidius. Appl Environ Microbiol 77: 1918–1920.
  21. 21. Dale C, Young SA, Haydon DT, Welburn SC (2001) The insect endosymbiont Sodalis glossinidius utilizes a type III secretion system for cell invasion. Proc Natl Acad Sci U S A 98: 1883–1888.
  22. 22. Cheng Q, Aksoy S (1999) Tissue tropism, transmission and expression of foreign genes in vivo in midgut symbionts of tsetse flies. Insect Mol Biol 8: 125–132.
  23. 23. Runyen-Janecky LJ, Brown AN, Ott B, Tujuba HG, Rio RV (2010) Regulation of high-affinity iron acquisition homologues in the tsetse fly symbiont Sodalis glossinidius. J Bacteriol 192: 3780–3787.
  24. 24. Pontes MH, Babst M, Lochhead R, Oakeson K, Smith K, et al. (2008) Quorum sensing primes the oxidative stress response in the insect endosymbiont, Sodalis glossinidius. PLoS One 3: e3541.
  25. 25. Matthew CZ, Darby AC, Young SA, Hume LH, Welburn SC (2005) The rapid isolation and growth dynamics of the tsetse symbiont Sodalis glossinidius. FEMS Microbiol Lett 248: 69–74.
  26. 26. Toh H, Weiss BL, Perkin SA, Yamashita A, Oshima K, et al. (2006) Massive genome erosion and functional adaptations provide insights into the symbiotic lifestyle of Sodalis glossinidius in the tsetse host. Genome Res 16: 149–156.
  27. 27. Belda E, Moya A, Bentley S, Silva FJ (2010) Mobile genetic element proliferation and gene inactivation impact over the genome structure and metabolic capabilities of Sodalis glossinidius, the secondary endosymbiont of tsetse flies. BMC Genomics 11: 449.
  28. 28. Aksoy S (1995) Wigglesworthia gen. nov. and Wigglesworthia glossinidia sp. nov., taxa consisting of the mycetocyte-associated, primary endosymbionts of tsetse flies. Int J Syst Bacteriol 45: 848–851.
  29. 29. Cheng Q, Ruel TD, Zhou W, Moloo SK, Majiwa P, et al. (2000) Tissue distribution and prevalence of Wolbachia infections in tsetse flies, Glossina spp. Med Vet Entomol 14: 44–55.
  30. 30. O’Neill SL, Gooding RH, Aksoy S (1993) Phylogenetically distant symbiotic microorganisms reside in Glossina midgut and ovary tissues. Med Vet Entomol 7: 377–383.
  31. 31. Lindh JM, Lehane MJ (2011) The tsetse fly Glossina fuscipes fuscipes (Diptera: Glossina) harbours a surprising diversity of bacteria other than symbionts. Antonie Van Leeuwenhoek 99: 711–720.
  32. 32. Wu D, Daugherty SC, Van Aken SE, Pai GH, Watkins KL, et al. (2006) Metabolic complementarity and genomics of the dual bacterial symbiosis of sharpshooters. PLoS Biol 4: e188.
  33. 33. McCutcheon JP, Moran NA (2007) Parallel genomic evolution and metabolic interdependence in an ancient symbiosis. Proc Natl Acad Sci U S A 104: 19392–19397.
  34. 34. Akman L, Yamashita A, Watanabe H, Oshima K, Shiba T, et al. (2002) Genome sequence of the endocellular obligate symbiont of tsetse flies, Wigglesworthia glossinidia. Nat Genet 32: 402–407.
  35. 35. Snyder AK, Deberry JW, Runyen-Janecky L, Rio RV (2010) Nutrient provisioning facilitates homeostasis between tsetse fly (Diptera: Glossinidae) symbionts. Proc Biol Sci 277: 2389–2397.
  36. 36. Rio RV, Symula RE, Wang J, Lohs C, Wu YN, et al. (2012) Insight into the transmission biology and species-specific functional capabilities of tsetse (Diptera: glossinidae) obligate symbiont Wigglesworthia. MBio 3.
  37. 37. Buchner P (1965) Endosymbiosis of animals with plant microorganisms. New York: Interscience Publishers.
  38. 38. Krieg NR, Hoffman PS (1986) Microaerophily and oxygen toxicity. Annu Rev Microbiol 40: 107–130.
  39. 39. Coombes BK (2009) Type III secretion systems in symbiotic adaptation of pathogenic and non-pathogenic bacteria. Trends Microbiol 17: 89–94.
  40. 40. Dale C, Jones T, Pontes M (2005) Degenerative evolution and functional diversification of type-III secretion systems in the insect endosymbiont Sodalis glossinidius. Mol Biol Evol 22: 758–766.
  41. 41. Hueck CJ (1998) Type III protein secretion systems in bacterial pathogens of animals and plants. Microbiol Mol Biol Rev 62: 379–433.
  42. 42. Dale C, Plague GR, Wang B, Ochman H, Moran NA (2002) Type III secretion systems and the evolution of mutualistic endosymbiosis. Proc Natl Acad Sci U S A 99: 12397–12402.
  43. 43. Moran NA, Degnan PH, Santos SR, Dunbar HE, Ochman H (2005) The players in a mutualistic symbiosis: insects, bacteria, viruses, and virulence genes. Proc Natl Acad Sci U S A 102: 16919–16926.
  44. 44. Cirillo DM, Valdivia RH, Monack DM, Falkow S (1998) Macrophage-dependent induction of the Salmonella pathogenicity island 2 type III secretion system and its role in intracellular survival. Mol Microbiol 30: 175–188.
  45. 45. Verbarg S, Fruhling A, Cousin S, Brambilla E, Gronow S, et al. (2008) Biostraticola tofi gen. nov., spec. nov., a novel member of the family Enterobacteriaceae. Curr Microbiol 56: 603–608.
  46. 46. Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ (1990) Basic local alignment search tool. J Mol Biol 215: 403–410.
  47. 47. Pontes MH, Smith KL, De Vooght L, Van Den Abbeele J, Dale C (2011) Attenuation of the sensing capabilities of PhoQ in transition to obligate insect-bacterial association. PLoS Genet 7: e1002349.
  48. 48. Hall T (1999) BioEdit: a user-friendly biological sequence alignment editor and analysis program for Windows 95/98/NT. Nucleic Acids Symp Ser. pp. 95–98.
  49. 49. Katoh K, Kuma K, Toh H, Miyata T (2005) MAFFT version 5: improvement in accuracy of multiple sequence alignment. Nucleic Acids Res 33: 511–518.
  50. 50. Castresana J (2000) Selection of conserved blocks from multiple alignments for their use in phylogenetic analysis. Mol Biol Evol 17: 540–552.
  51. 51. Guindon S, Delsuc F, Dufayard JF, Gascuel O (2009) Estimating maximum likelihood phylogenies with PhyML. Methods Mol Biol 537: 113–137.
  52. 52. Guindon S, Gascuel O (2003) A simple, fast, and accurate algorithm to estimate large phylogenies by maximum likelihood. Syst Biol 52: 696–704.
  53. 53. Huelsenbeck JP, Ronquist F (2001) MRBAYES: Bayesian inference of phylogenetic trees. Bioinformatics 17: 754–755.
  54. 54. Ronquist F, Huelsenbeck JP (2003) MrBayes 3: Bayesian phylogenetic inference under mixed models. Bioinformatics 19: 1572–1574.
  55. 55. Nylander JA, Wilgenbusch JC, Warren DL, Swofford DL (2008) AWTY (are we there yet?): a system for graphical exploration of MCMC convergence in Bayesian phylogenetics. Bioinformatics 24: 581–583.
  56. 56. Abascal F, Zardoya R, Posada D (2005) ProtTest: selection of best-fit models of protein evolution. Bioinformatics 21: 2104–2105.
  57. 57. Posada D (2008) jModelTest: phylogenetic model averaging. Mol Biol Evol 25: 1253–1256.
  58. 58. Mitsuhashi JM, Maramorosch K (1964) Leafhopper tissue culture: embryonic, nymphal and imaginal tissue from aseptic insects. Contribution from Boyce Thompson Institute. pp. 435–460.
  59. 59. Dale C, Beeton M, Harbison C, Jones T, Pontes M (2006) Isolation, pure culture, and characterization of “Candidatus Arsenophonus arthropodicus,” an intracellular secondary endosymbiont from the hippoboscid louse fly Pseudolynchia canariensis. Appl Environ Microbiol 72: 2997–3004.
  60. 60. Igarashi A (1978) Isolation of a Singh’s Aedes albopictus cell clone sensitive to Dengue and Chikungunya viruses. J Gen Virol 40: 531–544.