We sequenced the genome of Rickettsia felis, a flea-associated obligate intracellular α-proteobacterium causing spotted fever in humans. Besides a circular chromosome of 1,485,148 bp, R. felis exhibits the first putative conjugative plasmid identified among obligate intracellular bacteria. This plasmid is found in a short (39,263 bp) and a long (62,829 bp) form. R. felis contrasts with previously sequenced Rickettsia in terms of many other features, including a number of transposases, several chromosomal toxin–antitoxin genes, many more spoT genes, and a very large number of ankyrin- and tetratricopeptide-motif-containing genes. Host-invasion-related genes for patatin and RickA were found. Several phenotypes predicted from genome analysis were experimentally tested: conjugative pili and mating were observed, as well as β-lactamase activity, actin-polymerization-driven mobility, and hemolytic properties. Our study demonstrates that complete genome sequencing is the fastest approach to reveal phenotypic characters of recently cultured obligate intracellular bacteria.
Citation: Ogata H, Renesto P, Audic S, Robert C, Blanc G, Fournier P-E, et al. (2005) The Genome Sequence of Rickettsia felis Identifies the First Putative Conjugative Plasmid in an Obligate Intracellular Parasite. PLoS Biol 3(8): e248. doi:10.1371/journal.pbio.0030248
Academic Editor: Nancy Moran, University of Arizona, United States of America
Received: March 8, 2005; Accepted: May 11, 2005; Published: July 5, 2005
Copyright: © 2005 Ogata et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
Competing interests: The authors have declared that no competing interests exist.
Abbreviations: HEPN, higher eukaryotes and prokaryotes nucleotide-binding domain; MFS, major facilitator superfamily; Mpf, mating pair formation; ORF, open reading frame; PBS, phosphate-buffered saline; PCR, polymerase chain reaction; (p)ppGpp, guanosine tetra- and pentaphosphates; RPE, Rickettsia palindromic element; RT-PCR, reverse transcriptase–polymerase chain reaction; SFG, spotted-fever group; TPR, tetratricopeptide repeat; T4SS, type IV secretion system; XTC cell, Xenopus laevis tissue culture cell
Rickettsiae are obligate intracellular small gram-negative bacteria associated with different arthropod hosts. Many Rickettsia species infect human beings and are responsible for mild to severe diseases. Rickettsia felis, the agent of the flea-borne spotted fever rickettsiosis, exhibits several specificities among the currently recognized Rickettsia species. After being identified in fleas in 1990 , R. felis has been found worldwide in flea species such as Ctenocephalides felis, parasitizing cats and dogs, and Pulex irritans. R. felis is transovarially transmitted in these insects . Several cases of human infection caused by R. felis have been reported [3,4]. Rickettsia species are phylogenetically classified into two groups: the typhus group and the spotted-fever group (SFG). R. felis belongs to the SFG, together with tick-associated Rickettsia species such as R. conorii, R. sibirica, and R. rickettsii. However its lifestyle resembles that of R. typhi (typhus group), which is also hosted and transovarially transmitted by fleas. Furthermore, R. felis is known to coinfect fleas with Bartonella henselae, B. quintana, and Wolbachia pipientis . The culture conditions of R. felis were established in 2001 using Xenopus laevis tissue culture (XTC) cells at relatively low temperatures (optimally at 28 °C) . Besides these features, little is known about this pathogen. To date, six Rickettsia genome sequences are available. These are from two typhus group species (R. prowazekii  and R. typhi ) and four SFG species (R. conorii , R. sibirica , R. rickettsii, and R. akari). To further identify the specificities of R. felis, we determined its genome sequence.
General Genome Features
The genome of R. felis comprises three replicons: a 1,485,148 bp circular chromosome and two circular plasmids identified for the first time in the genus Rickettsia (Figure 1). The predicted total complement of 1,512 protein-coding genes (open reading frames [ORFs]) is the largest among currently sequenced Rickettsia genomes (Table 1). Of these, 1,402 (92.7%) exhibited homologs in the nonredundant database and 1,080 (71.4%) were assigned putative functions.
The three outer circles represent the chromosomes of R. felis, R. conorii, and R. prowazekii, respectively, with specific ORFs colored in red and nonspecific ORFs colored in black. Colinear genome fragments are highlighted by a shared background color, with their relative orientations indicated by arrows. The two inner circles represent two R. felis plasmids (pRF and pRFδ), with ORFs in the region unique to pRF colored in red.
The R. felis chromosome exhibits a long-range (24−277 kbp) colinearity relative to other Rickettsia genomes, although it is more frequently interrupted by inversions/translocations than is observed between other Rickettsia genomes (Figure 2A). This colinearity allowed the precise assessment of orthologous relationships between ORFs of five Rickettsia species (R. felis, R. conorii, R. sibirica, R. prowazekii, and R. typhi). On this basis, we identified 530 R. felis–specific ORFs, that were either absent or degraded (split or fragmented) in the other four Rickettsia genomes (Tables 2 and 3). Consistently, the R. felis genome exhibited a much higher number of gene families than other Rickettsia species (see Table 1). The R. felis–specific ORFs included a remarkably high number of paralogs for transposases, surface cell antigens (sca), global metabolism regulators (spoT), and proteins containing protein–protein interaction motifs such as ankyrin repeats and tetratricopeptide repeats (TPRs). Furthermore, we identified many other ORFs putatively associated with the adaptations of R. felis to its host environment or with its pathogenesis.
Red dots represent homologous genomic segments greater than 150 bp identified by BLASTN (E-value < 10−3).
(A) Comparison between R. felis and R. conorii chromosomes. Vertical and horizontal green lines indicate the positions of transposase ORFs in R. felis and in R. conorii, respectively.
(B) Self-comparison of R. felis chromosome.
The two R. felis plasmids, named pRF and pRFδ, are 62,829 bp and 39,263 bp long, respectively. Their topologies and sizes were confirmed experimentally (Figures S1 and S2). The pRF plasmid contains 68 ORFs, of which 53 (77.9%) exhibited homologs in public databases and 44 (64.7%) were associated with functional attributes. The nucleotide sequences of pRFδ and pRF are identical, except for an additional 23,566-bp segment that contains 24 ORFs (pRF15–pRF38) in pRF (see Table 3). These plasmids are likely to be R. felis specific since all attempts to detect specific plasmid sequences by polymerase chain reaction (PCR) from DNA of available reference rickettsial species were unsuccessful. In contrast, the same assays against 30 fleas naturally infected by R. felis resulted in amplification of the plasmid sequences in all cases.
Plasmids are referred to as conjugative or nonconjugative. The former are disseminated by conjugation from cell to cell, while the latter are only vertically transmitted. The pRF plasmid encodes several homologs of proteins involved in the different conjugative steps (see Table 3; Figure S3). First, it exhibits a split gene (pRF38/pRF39) homologous to the traATi of the Agrobacterium tumefaciens tumor-inducing plasmid . TraATi is thought to be a DNA-processing machinery with nickase and helicase activities to generate the transfer strand from the origin of transfer (oriT) . Second, the pRF encodes another split gene (pRF43/pRF44) homologous to the traDF in the Escherichia coli F plasmid. TraDF is a “coupling protein” that connects the DNA-processing machinery (and transfer strand) to the mating pair formation (Mpf) apparatus, a type IV secretion system (T4SS) . Finally, pRF exhibits an ORF (pRF47) similar to TraGF, a protein involved in the F-pilus assembly and aggregate stabilization .
Despite the presence of these ORFs linked to the initiation of plasmid transfer, the pRF sequence lacks clear homologs for the proteins involved in the Mpf apparatus found in other bacteria. Nevertheless, the R. felis chromosome (as well as other Rickettsia genomes) encodes most of the components of T4SS, which are highly similar to the vir genes of A. tumefaciens. Since the R. felis T4SS components (virB2 [RF1075], virB3 [RF0087], virB4 [RF0088], virB6 [RF0089, RF0090, RF0091, RF0092, and RF0093], virB8 [RF0463 and RF0465], virB9 [RF0462 and RF0466], virB10 [RF0467], virB11 [RF0468], and virD4 [RF0469]) are conserved in all sequenced Rickettsia genomes that lack plasmids, the primary suspected role of the R. felis T4SS is to translocate virulence factors to hosts. However, the T4SS of A. tumefaciens (vir) and Legionella pneumophila (dot/icm) have been shown to function both as DNA-transfer machineries and as effector translocators . Thus, the R. felis T4SS may also promote the transfer of DNA as in A. tumefaciens. We also noticed that the R. felis chromosome exhibits a DNA primase gene (RF0786) similar to TraC found in the E. coli IncP plasmid. TraC initiates the replication of transferred DNA strands in the recipient cells. Finally, the R. felis chromosome encodes a protein (RF0020) similar to competence protein ComE3, a protein (RF0964) similar to the F-pilin acetylation protein TraX, and a split gene (RF0705/RF0706) homologous to the P-pilus assembly protein FimD. In conclusion, the presence of those putative conjugative transfer genes suggests that the R. felis plasmids have been acquired by conjugation and that R. felis may still retain the capacity of transferring plasmids.
We identified 333 repeated DNA sequences (50 to 2,645 bp long) in the R. felis genome, accounting for 4.3% of the sequence, a proportion markedly higher than in other sequenced Rickettsia genomes (see Table 1; Figure 2B). The major source of those repeats is the proliferation of transposase genes, for which we identified 82 copies (or inactivated derivatives). Among other obligate intracellular bacteria, only W. pipientis wMel  and Parachlamydia sp. UWE25  exhibit such a high number of large mobile genetic elements. The occurrence of highly similar transposase sequences appears to play a major role in the plasticity of the R. felis genome (see Figure 2A). Transposase ORFs were identified at most extremities of the R. felis genomic segments colinear with the R. conorii genome, suggesting that the R. felis chromosome has been rearranged many times through recombination mediated by these mobile sequences. With the use of the GRAPPA software inferring the most parsimonious genome-rearrangement scenario, we estimated at least 11 inversion events between R. felis and R. conorii. In contrast, only four inversions are required to associate more distantly related R. conorii and R. prowazekii genomes. In addition to transposases, we identified eight phage-related ORFs (see Table 2). The R. felis genome thus appears to have been invaded more frequently by such foreign DNAs than other Rickettsia species. Besides long repeats, Rickettsia genomes are known to contain a number of small palindromic repeats (Rickettsia palindromic elements [RPEs]) capable of invading both coding and noncoding regions . We identified 728 RPEs in the R. felis genome. Of these RPEs, 85 were found within ORFs and three were found in RNA-coding genes.
The R. felis chromosome and plasmids share several homologs, suggesting gene exchanges between these replicons. Of 68 ORFs in pRF, 11 have a close homolog (>50% amino acid sequence identity) in the chromosome; these are seven transposases, patatin-like phospholipase (pRF11), thymidylate kinase (pRF13), and two small heat-shock proteins (pRF51 and pRF52). Among these, patatin-like proteins exhibit the most intriguing phylogeny (Figure S4). The genomes of five Rickettsia species (R. prowazekii, R. typhi, R. conorii, R. sibirica, and R. felis) exhibit chromosomal patatin-like phospholipase gene (pat1). Gene organization around pat1 is similar between these Rickettsia. Interestingly, a phylogenetic analysis for these Pat1 and the plasmid-encoded Pat2 indicates a close relationship between Pat1 (RF0360) and Pat2 of R. felis, together being an outgroup of Pat1 sequences of other Rickettsia, suggesting a gene replacement of the chromosomally encoded pat1 by the plasmid-encoded pat2 in the lineage leading to R. felis.
Most R. felis genes with orthologs in other Rickettsia have probably been inherited vertically from a common ancestor. On the other hand, genes without orthologs in other Rickettsia may have been acquired by lateral gene transfer. To test this hypothesis, we analyzed the taxonomic distribution of BLASTP best hits of R. felis ORFs against the nonredundant database (excluding rickettsial sequences) (Figure S5). R. felis ORFs with orthologs in other Rickettsia matched preferentially (64%) with sequences from the same taxonomic group as R. felis (i.e., α-proteobacteria). In contrast, the BLAST best hits for the chromosomal ORFs lacking orthologs in other Rickettsia were found preferentially in γ-proteobacteria (31%; 58 ORFs) and cyanobacteria (18%; 33 ORFs). The taxonomic distributions of the best matches for these two ORF sets were significantly different (p < 0.001; χ2 test). This result suggests that many R. felis-specific genes may originate from distantly related organisms by lateral transfer. However, methods based on nucleotide composition bias failed to identify unambiguous candidates for lateral gene acquisition in R. felis.
The sca family is one of the largest paralogous gene families in Rickettsia . Five sca members have been identified in the previously published Rickettsia genomes. Several Sca proteins are known to account for major antigenic differences between Rickettsia species  and may play important roles in adhesion to host cells . Sca proteins are characterized by highly variable N-terminal sequences and a conserved C-terminal autotransporter β-domain, which translocates the N-terminal part outside the outer membrane. The R. felis genome exhibits the highest number of sca genes among currently available Rickettsia genomes. We identified nine intact sca paralogs (sca1, sca2, sca3, sca4, sca5/ompB, sca8, sca9, sca12, and sca13) as well as four fragmented or split paralogs (sca0/ompA, sca7, sca10, and sca11). Reverse transcriptase–polymerase chain reaction (RT-PCR) experiments demonstrated that, under mild log growth phase, all R. felis sca paralogs were transcribed, including split ones. Phylogenetic analyses suggest that ancient duplication events gave rise to these paralogs before the divergence of Rickettsia species. We noticed that sca genes exhibit highly different patterns of presence/absence across different Rickettsia species (Table S1). Only ompB and sca4 are conserved in all available Rickettsia genomes , remaining members being degraded or absent in one or more species. Together with the accelerated amino acid changes, differential gene degradation of sca paralogs probably contributes to the intra-species variation of those cell-surface proteins and might be linked with their adaptation to different host environments.
R. felis is genetically and serologically classified into the SFG of Rickettsia . However, cross-reactivities caused by both proteins and lipopolysaccharides have been found with R. typhi using mouse sera  and human sera (Figure S6). R. conorii rarely cross-reacts with R. typhi. We therefore suspected that genes found in both R. felis and R. typhi, but missing in R. conorii, might be responsible for the cross-reactivities of R. felis and R. typhi. A list of such genes includes a sca family gene (sca3), encoding a protein with a predicted molecular weight of 319 kDa, and rfaJ for the lipopolysaccharide 1,2-glucosyltransferase (Table 4).
Adaptation to Environment
Transcriptional regulation may be of critical importance in R. felis, as the numbers of spoT, the gene regulating “alarmone,” and chromosomal toxin–antitoxin modules are higher in the R. felis genome than in any other sequenced bacterial genome.
SpoT and RelA are two hallmark enzymes regulating global cellular metabolism of E. coli in response to starvation . These enzymes control the concentration of alarmone, (p)ppGpp (guanosine tetra- and pentaphosphates), which in turn acts as an effector of transcription. Remarkably, R. felis exhibits 14 spoT, (spoT1–13 and 15) paralogs (Figure S7). Using RT-PCR, we examined the transcription status of 14 R. felis spoT genes. All the spoT ORFs were transcribed. We classified these ORFs into two groups, based on their alignment against the sequence of the Streptococcus dysgalactiae Relseq that possesses both (p)ppGpp hydrolase and synthetase activities . The first group (SpoT1–10, 14, and 15) was aligned with the sequence of the hydrolase domain, and the second group (SpoT11, 12, and 13) with the sequence of the synthetase domain. Being consistent with the previous observation , our phylogenetic analyses suggest that each paralogous gene group originated in early duplication events before the divergence of Rickettsia species. Notably, every sequenced Rickettsia genome encodes at least one ORF exhibiting hydrolase catalytic residues and one ORF exhibiting synthetase catalytic residues, suggesting that both hydrolase and synthetase functions are required for Rickettsia. We also found that seven spoT(spoT1–4 and 7–9) genes were located in the R. felis chromosome next to a gene encoding a transporter of the major facilitator superfamily (MFS) including proline/betaine transporters. MFS is also a large paralogous gene family composed of at least 23 ORF members in R. felis.
Toxin–antitoxin systems are composed of tightly linked toxin and antitoxin gene pairs and ensure stable plasmid inheritance when they are encoded in plasmids. In these systems, the toxic effect of a long-lived toxin is continuously inhibited by a short-lived antitoxin only when whole systems are maintained. The toxin–antitoxin modules have also been found on the chromosomes of many free-living prokaryotes, but have rarely been found in obligate intracellular bacteria [24,25]. In the R. felis chromosome, we identified 16 toxin genes (RF0016, RF0095, RF0271, RF0456, RF0490, RF0602, RF0701, RF0732, RF0787, RF0792, RF0898, RF0911, RF0956, RF1272, RF1286, and RF1368) and 14 antitoxin genes (RF0015, RF0094, RF0272, RF0457, RF0489, RF0601, RF0702, RF0731, RF0779, RF0788, RF0899, RF0910, RF0957, and RF1369), comprising at least 13 modules in operon structures. It is suggested that toxin–antitoxin systems, when encoded on the bacterial chromosome, might be involved in selective killing (a primitive form of bacterial apoptosis) or reversible stasis of bacterial subpopulations during periods of starvation or other stress [26,27]. It is also tempting to speculate that the toxin–antitoxin system could be targeted to the eukaryotic host cells. In this case, this system may help to maintain the presence of bacteria in the host. Notably, in the chromosomally encoded mazEF system of E. coli, the toxin action is regulated by (p)ppGpp. The large number of toxin–antitoxin modules in R. felis, as well as a number of spoT paralogs, might thus be linked to the synchronization of its multiplication within eukaryotic hosts.
It is probable that five R. felis–specific ORFs are related to its capacity of antibiotic resistance. We identified a streptomycin resistance protein homolog (RF0774), a class C β-lactamase, AmpC (RF1367), a class D β-lactamase (RF1275), a penicillin acylase homolog with conserved catalytic residues (RF1137), and an ABC-type multidrug transport-system protein, MdlB (RF0981). AmpC β-lactamase is known to be induced by AmpG of the MFS, which was also identified in the R. felis genome (RF0265, RF0608, RF0834, and RF1247). In vivo β-lactamase activity of R. felis was measured using high-performance liquid chromatography (see below).
Adaptation to Eukaryotic Hosts
R. felis may have developed a specific mechanism to cross-talk with its eukaryotic hosts. It exhibits 22 ankyrin-repeat-containing proteins and 11 TPR-containing proteins. These two protein motifs are frequently found in eukaryotic proteins, but their distributions are rather limited in viruses and bacteria, in both of which they appear to be linked with pathogenicity.
The ankyrin repeat is a protein–protein interaction motif, involved in transcription initiation, cell cycle regulation, cytoskeletal integrity, and cell-to-cell signaling . Anaplasma phagocytophilum, a closely related intracellular α-proteobacterium, exhibits a protein containing ankyrin repeats (AnkA), which was detected in the cytoplasm and the nucleus of infected eukaryotic cells (human leukemia-60) . According to the Superfamily database , only 15 bacterial species possess more than three ankyrin-repeat-containing proteins, and two species exhibiting the highest number of ankyrin repeats are obligate intracellular bacteria, W. pipientis (21 proteins) and Coxiella burnetii (20 proteins), although Wu et al.  reported slightly different numbers of ankyrin-repeat-containing proteins for these species. A recent genome analysis of a facultative intracellular bacterium, L. pneumophila, revealed 20 proteins with ankyrin repeats . Ankyrin repeats were also found in more than 30 ORFs of the giant virus Acanthamoeba polyphaga Mimivirus .
TPR, composed of a motif of 34 amino acids organized in tandem, is also recruited by different proteins and facilitates protein–protein interactions . Its role in the adaptation of parasites to their hosts has been suggested. The R. felis genome exhibits 11 TPR-containing ORFs (seven in the chromosome and four in the pRF plasmid). Only Leptospira interrogans (the agent of leptospirosis), Treponema species (including the agent of syphilis), and L. pneumophila  exhibit a high number of both TPR and ankyrin repeats. These organisms are eukaryotic parasites. The cryptococcal crooked neck 1 gene of Cryptococcus neoformans (a yeast), containing 16 copies of TPR, appears associated with its virulence .
Plasmids often carry out functions that benefit bacteria in their survival or expression of virulence. pRF exhibits two ORFs that are possibly associated with the pathogenesis of R. felis: a hyaluronidase and a patatin-like protein. The hyaluronidase homolog (pRF56) exhibits a significant homology to hyaluronidase NagI (1,297 aa) of Clostridium perfringens. Hyaluronidases, which depolymerize hyaluronic acid—an unbranched polysaccharide ubiquitously present in the extracellular matrix of animal tissues—are known as “spreading factors” . Another ORF (pat2) exhibits a significant homology to patatin-like phospholipases. Its paralog (pat1) was also identified in the chromosome, as already mentioned. Patatin is the major storage glycoprotein found in potato tubers, but also exhibits phospholipase A2 activity for protection from infection. Proteins containing patatin-like domains are more frequently found in pathogenic than in nonpathogenic bacteria. McLeod et al.  suggested that patatin-like proteins might be responsible for the phospholipase A2 activity identified some years ago in rickettsiae .
Potential host-invasion capacity is also provided by R. felis–specific ORFs found on the chromosome, for instance, a chitinase homolog (RF0413) and a chitin-binding protein homolog (RF0710). Chitin is a homopolymer of N-acetylglucosamine and a major component of the exoskeleton of arthropods and of the peritrophic envelope of insects, a lining layer of the midgut. These genes may facilitate the access of bacteria to the insects' gut epithelial cells. R. felis may also use chitin as a nutrient source, as does Vibrio cholerae . We identified a homolog (RF0268) for ecotin, an E. coli periplasmic protein inhibiting activities of a variety of proteases. Two R. felis–specific ORFs (RF0449 and RF0855) exhibit the complete NACHT NTPase domain. In eukaryotes, this NTPase domain has been found in proteins implicated in apoptosis as well as in immune/inflammatory responses . The presence of this domain in other bacterial ORFs is limited to several lineages, such as cyanobacteria and Streptomyces, and their functions are unknown.
Higher eukaryotes and prokaryotes nucleotide-binding domain (HEPN) is a recently identified domain detected in a few prokaryotes. We found four genes (two were split) exhibiting HEPN at the C-terminus, and a nucleotidyl transferase domain at the N-terminus. Among other bacteria, only A. tumefasciens, Thermotoga maritima, and Sinorhizobium melitoti were found to exhibit HEPN-containing genes . The nucleotidyl transferase domain has been associated with several classes of bacterial enzymes responsible for resistance to aminoglycosides. HEPN was also found in the human sacsin protein, a chaperonin implicated in a neurodegenerative disease. Finally, R. felis exhibits an ortholog (RF0371) for R. conorii RickA, which induces its actin-based motility .
Phenotypic Post-Genomics Analysis
The obligate intracellular nature of R. felis hindered progress in the detailed characterization of its phenotypic diversity. Here, we envisaged post-genomics as a way of associating in vivo phenotypes of these bacteria to genomic features. The presence of pili-associated genes prompted us to investigate, by electron microscopy, the presence of such appendages on the cell surface. This approach led to the first characterization of pili on the surface of a Rickettsia; we observed two forms of pili at the surfaces of R. felis (Figure 3). One form of pili establishes direct contact between bacteria, providing a very typical figure of Mpf apparatus; these pili are probably specialized in conjugation. The other form of pili forms small hair-like projections emerging out from the cell surface; these pili are probably involved in the attachment of the bacteria to other cells. Without pili, many disease-causing bacteria lose their invasion capability. The latter type of pili might be considered as virulence factors, as described for Francisella tularensis [41,42].
Bacteria collected from the supernatant of R. felis–infected XTC cells were negatively stained.
(A) Sexual pilus observed between two bacteria.
(B) R. felis also possesses small appendages likely to be fimbriae pili.
As previously mentioned, we also found a RickA homolog in the R. felis genome . Based on this finding, we performed immunofluorescence assays. The orientations of actin filaments beside bacteria are distinct from the stress fibers of the host. This further suggests that R. felis is probably capable of using the actin cytoskeleton to disseminate through eukaryotic cells, a method exploited by other SFG rickettsiae  (Figure S8). Another R. felis phenotypic character suggested from genomic analyses (three ORFs for patatin-like proteins) was its hemolytic capacity. We confirmed experimentally that R. felis lyses erythrocytes, this effect being inhibited by dithiothreitol. Another genome-guided discovery was β-lactam inhibition, which reached 57% and 53% of the concentration and the minimal inhibitory concentration, respectively, following 2 h incubation of R. felis with amoxicillin. Despite being preliminary results, these findings illustrate the fact that whole-genome sequencing offers opportunities to rapidly gain a better understanding of the phenotypic characters of a fastidious microorganism.
R. felis is the first obligate intracellular bacterium exhibiting a possible conjugative plasmid. Of the nine previously published studies of members of the Order Rickettsiales (six in Rickettsiaceae, three in Anaplasmateceae), none exhibited a plasmid. Several other obligate intracellular bacteria, such as Chlamydia muridarum, Chlamydophila caviae, C. burnetii, Wigglesworthia glossinidia, and Buchnera aphidicola, are known to possess plasmids. Recently, the reannotation of the genome of Parachlamydia, an obligate intracellular bacteria living in amoeba, predicted an F-like DNA conjugative system encoded in a genomic island . However, no conjugation has yet been observed for those plasmids and genomic island. Transformation of obligate intracellular bacteria remains an elusive goal, although preliminary work on several obligate intracellular bacteria has been reported with limited results . The possible conjugative plasmid identified in R. felis may provide a molecular basis for the future development of new genetic transformation tools in rickettsiae.
R. felis is hosted by fleas, as are R. typhi, B. henselae, W. pipientis, and Yersinia pestis. There are surprisingly few common genomic features between R. typhi and R. felis. R. typhi genetically resembles R. prowazekii despite having a lifestyle similar to that of R. felis (Table S2). The comparison with W. pipientis is interesting. This intracellular bacterium also multiplies in arthropods (including fleas) and is transmitted transovarially. The most relevant finding in its genome was the detection of repetitive mobile DNA elements. Many ankyrin repeats and several TPRs were also found. It appears that R. felis and W. pipientis share common genomic features, possibly because of their similar niches (we found two Ct. felis fleas in France coinfected with W. pipientis and R. felis). They both differ significantly from their immediate neighbors [45,46]. Moreover, the phylogenetic relationship and hosts of R. felis and R. prowazekii (transmitted by lice) are comparable with those for B. quintana (transmitted by lice) and B. henselae (transmitted by fleas) . B. henselae exhibits a larger genome with more repeats and integrases than B. quintana. Y. pestis, transmitted by fleas, also exhibits many more insertion sequences than its close relative, Y. pseudotuberculosis . Altogether, flea-infecting bacteria appear to exhibit a specific evolution (i.e., more repeats, transposases, and/or integrases) compared with their non-flea-infecting neighbors.
For obligate intracellular bacteria such as rickettsiae, few phenotypic characters have been observed. To date, four intracellular bacterial genomes have been entirely sequenced, the procedure being completed in 7 y or less after their first identification or culture, including R. felis [14,15,49,50]. In the present study, the genome sequencing of R. felis provided evidence of the presence of conjugative plasmids, two types of pili, hemolytic activity, β-lactamase activity, and intracellular motility. We believe that for such recently identified/cultured fastidious organisms, complete genome sequencing is a very potent and timesaving strategy to identify unrecognized phenotypic properties.
Materials and Methods
Bacterial purification and DNA extraction
R. felis (strain California 2) was cultivated on XTC cells growing on RPMI with 5% fetal bovine serum, supplemented with 5 mM L-glutamine. The purification of the bacteria was performed by different steps. First, the bacteria were treated in the presence of 1% trypsine in K36 buffer for 1 h at 37 °C, then centrifuged and digested by DNAseI for 1 h at 37 °C to reduce the eukaryotic DNA contamination. The sample was loaded on a renograffin gradient and the bands of the purified bacteria were washed in K36, treated again by DNAseI. After inactivation with EDTA (50 mM), the bacteria were resuspended in TE, dispatched in 150-μl tubes and stored at −80 °C. Depending on this initial concentration, one or two tubes were diluted in 1 ml of TNE (10 mM Tris [pH 7.5], 150 mM NaCl, 2 mM EDTA) and incubated for 5 h at 37 °C in the presence of lysozyme (2 mg/ml). Lysis was performed for 2 h at 37 °C by adding 1% SDS and RNAseI (25 μg/ml). Overnight treatment with 1 mg/ml of proteinase K followed at 37 °C. After three phenol–chloroform extractions and alcoholic precipitation, the DNA was resuspended in 30 μl of TE and its concentration was estimated by agarose gel electrophoresis.
Pulsed-field agarose gel electrophoresis
The concentrated bacterial suspension was included in 1% (vol/vol) Incert agarose gel blocks (BMA, Rockland, Maryland, United States). The agarose blocks were digested by Proteinase K (1 mg/ml) (Eurobio Laboratories, Paris, France) in 1% lauroylsarcosine and 0.5 M EDTA (pH 8) (Sigma-Aldrich, St. Louis, Missouri, United States) for 24 h at 50 °C. Fresh Proteinase K was then added and the incubation was continued for 24 h. The blocks were then washed twice in TE (pH 7.6) for 30 min at room temperature. Proteinase K inactivation was performed through incubation in a 4% phenylmethylsulfonyl fluoride (MBI Fermentas, Burlington, Canada) solution for 1 h at 50 °C. This inactivation step was carried out twice. The blocks were then washed two to three times in TE and stored in 0.5 M EDTA (pH 8) at 4 °C. Before restriction enzyme digestion, the agarose blocks were equilibrated twice with TE for 15 min. Digestion was carried out for 4 h, then fresh enzyme was added and the incubation was continued overnight. The digested agarose blocks and molecular-weight markers (Low Range PFG Marker, Lambda Ladder PFG Marker [New England Biolabs, Beverly, Massachusetts, United States]) were equilibrated in 0.5× TBE (50 mM Tris, 50 mM boric acid, 1 mM EDTA).
Each agarose block was laid in a 1% PFEG agarose (Sigma-Aldrich) solution in 0.5× TBE. Pulsed-field gel electrophoresis was carried out on a CHEF-DR II device (Bio-Rad, Hercules, California, United States) under different electrophoresis conditions. The 1% agarose gel was run at 200 V using ramped pulse times from 1 to 5 s for 10 h to observe the pattern of small DNA fragments (2–48 kb). The migration was taking place under the following two consecutive conditions: (i) a ramping time from 3 to 10 s at 200 V for 12 h, with the pattern representative for 48- to 242-kb fragments, then (ii) a ramping time from 20 to 40 s at 180 V for 15 h, with the pattern representative for 145- to 610-kb fragments.
Shotgun of R. felis genome and sequencing strategy
Three shotgun genomic libraries were constructed by mechanical shearing of the genomic DNA using a Hydroshear device (GeneMachine, http://genome.nhgri.nih.gov/genemachine/). DNA fragments were blunt-ended using T4 DNA polymerase (New England Biolabs) and ligated to the BstXI adapter. Fragments of 3, 4.5, and 7 kb were separated on a preparative agarose gel (FMC BioProducts, Rockland, Maryland, United States), extracted with Qiaquick kit (Qiagen, Valencia, California, United States), and ligated into pCDNA2.1 (Invitrogen, Carlsbad, California, United States) for the two smaller inserts and into pCNS (a low copy number vector; C. R., unpublished data) for the largest one. DNA cloning was performed using electrocompetent E. coli DH10B Electromax cells (Invitrogen). Plasmid DNAs were purified and pools of 96 clones were analyzed by gel electrophoresis to validate the libraries. DNA sequencing of insert ends was carried out using Big Dye 3.1 terminator chemistry on an automated capillary ABI3700 sequencer (Applied Biosystems, Foster City, California, United States).
Sequences were analyzed and assembled into contigs using Phred, Phrap, and Consed software  taking all sequences into account. Sequences were considered valid when at least 75% of the nucleotides had a Phred score of more than 20. The finishing of the genome sequencing included only additional directed reactions that were performed on an ABI3100 sequencer. Two circular plasmid molecules of 63 and 38 kbp, respectively, were identified from the assembled sequences. On the chromosome, three small regions of 41, 155, and 64 bp failed by dropping of sequence. A number of parameters (DMSO, glycerol, hybridization, and elongation temperature) were tested one by one or were combined to sequence over these gaps. We finally succeeded with the association of another type of chemistry, D-rhodamine with 2 M betaine. We designed and used 420 primers (i) to close the sequencing gaps by walking either on shotgun subclones or on the chromosome and (ii) to improve sequence regions of low quality.
The integrity of the assembly was validated by comparing the restriction patterns obtained by pulsed-field gel electrophoresis with those deduced from the electronic consensus sequence. The selection of restriction enzymes was based on rare sites. We analyzed single digests of R. felis DNA. The main restriction enzymes used for these studies were ApaI, AfeI, FspI, and SbfI. This comparative study confirmed the predicted length of the R. felis DNA fragments.
The structures for pRF and pRFδ plasmids were controlled by specific primer amplifications (see Figure S1). Three PCRs were performed and the amplification results were in agreement with the expected hypothesis. These PCR results validate the two distinct plasmid forms (62.8 and 39 kbp, respectively). Meanwhile, a Southern blot was performed through a pulsed-field electrophoresis gel. Uncut genomic R. felis DNA and R. felis DNA digested by the restriction enzyme PvuI (corresponding to a unique site in the pRF-specific region) were analyzed. These blocks of DNA were loaded twice onto the gel with the molecular-weight markers: Lambda Marker (Bio-Rad) and Low Range PFG Marker (New England Biolabs) as described above, with a pulse time from 1 to 5 s for 12 h at 180 V. The gel was treated and transferred onto Hybond N+ (Amersham Biosciences, Little Chalfont, United Kingdom) with a vacuum blot. The DNA was fixed by heating for 2 h at 80 °C, and the membrane was cut into two pieces. Two probes were derived from two PCR products. The first, pRFh–pRFi (726 bp), was designed within the pRF-specific insert, and the second, pRFa–pRFg (251 bp), was designed to encompass the deletion site of the pRFδ. These two probes were labeled with dCTP32 and hybridized at 65 °C for 17 h on each membrane. Membranes were washed three times in 1× SSC and 0.1% SDS at 65 °C. The exposure time ranged from 6 h to overnight at −80 °C on ECL film. The hybridizations were clearly established on R. felis digested by PvuI and led to one signal with the pRFh–pRFi probe and two signals for the two plasmid structures with the pRFa–pRFg probe at a predicted molecular weight compatible with our prediction (see Figure S2).
We tested 30 samples of fleas naturally infected by R. felis obtained from different geographic areas (Algeria [11 fleas], France [15 fleas], and New Zealand [four fleas]) with three pairs of primers: (i) primers designed in the traD gene (pRF37F1/R1), (ii) primers in the pRF plasmid (pRFe–pRFf), and (iii) primers in the pRFδ plasmid (pRFa–pRFg). We confirmed positive PCR products of (i) 196 bp, (ii) 208 bp, and (iii) 251 bp for all the 30 cases.
We predicted protein-coding genes (ORFs) using SelfID  as previously described . tRNA genes were identified using tRNAscan-SE . Database searches were performed using BLAST programs  against Swiss-Prot/TrEMBL , the NCBI CDD database , and SMART . The number of transposases, ankyrin/TPR-containing genes, autotransporter domains, and integrases were computed using PSI-BLAST with NCBI/CDD entries related to those domains with an E-value threshold of 10−5. Repeated DNA sequences were identified with the use of RepeatFinder , by ignoring the sequence similarity between pRF and pRFδ. To identify Rickettsia palindromic elements, we used hidden Markov models  based on the previously identified RPE sequences .
By taking advantage of genome colinearity, we identified orthologous relationships of genes in R. felis, R. conorii, R. sibirica, R. prowazekii, and R. typhi with the use of Genomeview (S. Audic, unpublished software). Based on the gene orthology, we defined R. felis–specific ORFs, which were of one of the following three classes: Class I ORFs exhibiting no homologous ORFs in the other four Rickettsia genomes; Class II ORFs exhibiting homologous ORFs but no orthologous ORFs in the other four Rickettsia genomes; and Class III ORFs exhibiting orthologous ORFs in some or all of the other four Rickettsia, all of which exhibit degraded (split or fragmented) genes relative to the R. felis ORF. Plasmid-encoded ORFs were by definition classified into Class I or II. A gene composed of more than one ORF was defined as “split gene.” A gene composed of a single ORF whose length is shorter than 50% of the longest ortholog was defined as a “fragmented” ORF. We used T-Coffee  and MEGA  for multiple sequence alignment and phylogenetic tree analyses, respectively. The analyses of horizontal gene transfer were performed by BLAST search against the Swiss-Prot/TrEMBL nonredundant database, excluding rickettsial sequences, as well as by methods based on nucleotide composition bias [63,64]. We obtained the minimum number of inversions to associate a pair of Rickettsia genomes using GRAPPA release 2.0 .
Ultrastructural characterization of pili by electronic microscopy
R. felis cells were carefully collected from the supernatant of XTC cells infected for 5 d and grown at 28 °C. Following centrifugation (400 g, 10 min), bacteria were fixed for 1 h at 4 °C in glutaraldehyde (2.5% in phosphate-buffered saline [PBS]). Cells were then washed in PBS and placed on a carbon–formvar-coated 400-mesh copper grid (Electron Microscopy Sciences, Hatfield, Pennsylvania, United States) for 15 min then negatively stained with 2% phosphotungstic acid for 10 s, before analysis by electron microscopy (Philips Morgagni 268D, Philips Electronics, Eindhoven, the Netherlands).
Estimation of β-lactamase activity
To evaluate the level of β-lactamase activity, 104R. felis cells grown on XTC cells and then sonicated were mixed with amoxicillin to a final concentration of 20 μg/ml, and incubated for 2 h at 28 °C. The concentration of amoxicillin was measured in the R. felis + amoxicillin suspension as well as in a suspension of XTC cells without bacteria + amoxicillin, before and after incubation, using high-performance liquid chromatography. In addition, the minimum inhibitory concentrations of these four suspensions were estimated by growth inhibition of a Micrococcus luteus strain.
RNA extraction and RT-PCR
Approximately 6.5 × 105 bacteria were used to infect one 25-cm3 flask of confluent XTC cells maintained at 28 °C. Infected cells were harvested 48 h later, centrifuged (12,000 g, 10 min), and pellets were immediately frozen in liquid nitrogen before being stored at −80 °C. Total RNA was isolated by using the RNeasy Mini Kit (Qiagen) according to the manufacturer's instructions. At the end of the extraction procedure, all samples were treated with RNase-Free DNase Set (Qiagen) for 30 min. The concentration and quality of isolated RNA were determined with the Agilent 2100 bioanalyzer (Agilent Technologies, Englewood, New Jersey, United States). Aliquots of the DNase-treated total RNA samples were stored at −80 °C until use. RT-PCR was performed from 2 μl of RNA (25 μl final reaction volume) with the Superscript One-Step RT-PCR with Platinum Taq (Invitrogen). Possible DNA contamination was assessed with the Expand high-fidelity polymerase (Roche, Basel, Switzerland). Cycling conditions were 30 min at 50 °C, 5 min at 95 °C, and 40 cycles at 30 s at 95 °C, 30s at 50 °C, and 1 min at 72 °C, followed by a final extension cycle of 7 min at 72 °C. The RT-PCRs were conducted on the PTC-100 thermocycler (Bio-Rad). Amplification products were run on 2% (wt/vol) agarose gels, and the DNA was stained with ethidium bromide. The size of the PCR product was determined by comparison with DNA molecular-weight marker VI (Boehringer Ingelheim, Ingelheim, Germany).
Detection of F-actin and immunofluorescence staining
Vero cells grown to semiconfluence on glass coverslips were infected with R. felis for 24–48 h at 28 °C in a humidified CO2 incubator (5% CO2). Infected cells were then fixed for 1 h at 4 °C with formaldehyde (3% wt/vol in PBS supplemented with 1 mM MgCl2 and 1 mM CaCl2), washed three times in PBS, and then made permeable with 0.2% Triton X-100 in PBS for 1 min. After three washings in PBS, the coverslips were incubated for 1 h with a monoclonal anti–R. felis antibody. Bacteria were visualized by staining with anti-mouse-Alexa 594 antibody (1:300) and F-actin with FITC-phalloidin (1:250). The coverslips were mounted using Fluoprep (BioMérieux, Marcy-l'Etoile, France) and were examined with a confocal laser scanning microscope using a 100× oil immersion objective lens.
Human blood (10 ml) was centrifuged (1,500 g, 10 min), and after three PBS washings, erythrocytes were resuspended in 20 ml of PBS. This suspension (100 μl) was mixed with 800 μl of PBS and 100 μl of rickettsial suspension (106, 105, and 104 bacteria, respectively). In some experiments, rickettsiae were incubated for 1 h at 35 °C in the presence of 2 mM DTT. Complete hemolysis was determined by adding 900 μl of H2O to erythrocytes, and spontaneous hemolysis corresponded to control without bacteria. Following 3 h of incubation at 35 °C, the samples were fixed using paraformaldehyde (0.3% final concentration) and centrifuged. Hemoglobin release was estimated by measurement of the optical density of the supernatant at 545 nm. This experiment was performed in duplicate.
The sequences of the primers for PCR and RT-PCR are provided in Table S3.
Figure S1. Confirmation of Plasmid Topologies for pRF and pRFδ by PCR
(A) The locations of the three primer sets (pRFa–pRFb, pRFc–pRFd, and pRFa–pRFd) used to validate the presence of the two distinct plasmid forms are indicated.
(B) The result of the PCR assay with these primers. Two pairs of primers (pRFa–pRFg and pRfh–pRFi) used to obtain the probes for the Southern blot (see Figure S2), as well as another pair of primers (pRF37F1/R1) used in plasmid detection in fleas infected by R. felis, are also indicated in (A).
(1.5 MB TIF).
Figure S2. Characterization of R. felis Plasmids by Southern Blot
The two membranes (A and B) loaded with R. felis genomic DNA (#1/4) and R. felis DNA digested by PvuI (#2/3) were hybridized either by the probe pRFa–pRFg or by pRFh–pRFi.
(39 KB PDF).
Figure S3. A Model for the Conjugative Plasmid Transfer of R. felis
This model is based on gram-negative bacterial conjugation systems involving T4SS. Homologs responsible for different steps of conjugation were identified in the R. felis genome. DNA-processing machinery, plasmid-encoded pRF38/39 (TraATi); the coupling protein, plasmid-encoded pRF43/44 (TraDF) or chromosomally encoded virD4 (RF0469); Mpf apparatus, chromosomal genes for virB2 (RF1075), virB3 (RF0087), virB4 (RF0088), virB6 (RF0089, RF0090, RF0091, RF0092, and RF0093), virB8 (RF0463 and RF0465), virB9 (RF0462 and RF0466), virB10 (RF0467), and virB11 (RF0468); priming for DNA replication in the recipient cell, chromosomally encoded RF0786 (TraC).
(57 KB PDF).
Figure S4. Phylogenetic Trees for the Patatin-Like Proteins, Thymidylate Kinases, and Small Heat-Shock Proteins
Phylogenetic trees were constructed using the neighbor-joining method with Jones-Taylor-Thornton model.
(16 KB PDF).
Figure S5. Taxonomic Distribution of BLAST Best Hits of R. felis ORFs
R. felis ORFs were searched against the nonredundant database (excluding rickettsial sequences). The distribution difference between ORFs with rickettsial orthologs and ORFs lacking rickettsial orthologs remained significant even after the removal of transposase ORFs.
(16 KB PDF).
Figure S6. Cross-Reactivity of R. felis
Western immunoblot showing the preferential cross-reactivity of antibodies with R. felis and R. typhi in a patient with murine typhus (lanes a–c), and with R. felis and R. conorii in a patient with Mediterranean spotted fever (lanes d–f). Lanes a and d, R. conorii antigen; lanes b and e, R. typhi antigen; lanes c and f, R. felis antigen; MM, molecular mass.
(30 KB PDF).
Figure S7. Domain Structures and the Presence/Absence Patterns of spoT Genes in Different Rickettsia
With reference to the S. dysgalactiae Relseq, four (H: 53H, 77H, 78D, and 144D) and five (241R, 243K, 251K, 264D, and 323E) catalytic residues were examined for the (p)ppGpp hydrolase and synthetase domains, respectively. ORF sizes were those for R. felis genes, except SpoT14, for which the R. prowazekii ORF size is indicated. a, absent; Ch, conserved hydrolase catalytic residues; Cs, conserved synthetase catalytic residues; s, split or fragmented genes.
(17 KB PDF).
Figure S8. Confocal Laser Analysis of R. felis–Infected Vero Cells
Bacteria were stained by indirect immunofluorescence using a monoclonal anti–R. felis antibody followed by an anti-mouse-Alexa 594 antibody (red). F-actin was stained with FITC-phalloidin (green). Arrows indicate R. felis with actin tail.
(29 KB PDF).
Table S1. Distribution of sca Genes among Rickettsia Genomes
(30 KB DOC).
Table S2. Comparison of Different Features of Bacteria Infecting Fleas with Their Close Relatives
(32 KB DOC).
Table S3. Nucleotide Sequences of the Primers Used in the Present Study
(28 KB DOC).
The genome sequence of R. felis is accessible via GenBank (http://www.ncbi.nlm.nih.gov/Genbank) under the accession numbers: CP000053, CP000054, and CP000055. The EMBL Nucleotide Sequence Database (http://www.ebi.ac.uk/embl) accession number for Cl. perfringens NagI is Q8XM09. The Pfam (http://www.sanger.ac.uk/Software/Pfam/) accession number for ComE3 is PF03772. The Protein Data Bank (http://www.rcsb.org/pdb/) accession number for S. dysgalactiae Relseq is 1VJ7.
We wish to thank Jean Weissenbach and his team at Genoscope for the shotgun sequencing, Bernadette Giumelli and Thi Tien N. Guyen for technical assistance in sequencing of the R. felis genome, Bernard Campagna for electronic microscopy analysis, Sylvianne Robineau for RT-PCR experiments, Claude Nappez for production of monoclonal antibodies against R. felis, and Deborah Byrne for carefully reading the manuscript. We gladly acknowledge the financial support of Marseille-Nice Genopole.
HO performed genome annotation and coordinated the bioinformatics analyses. PR performed electron microscopic analysis of pili, immunofluorescence assay of actin-based motility, and hemolytic activity assay. SA and CR assembled genome sequences, performed sequence finishing, and carried out experiments to characterize the plasmids. CR constructed genomic libraries. GB performed most phylogenetic analyses. PEF performed β-lactamase activity assay and contributed to the bioinformatics analyses. HP contributed to the sequencing. JMC provided laboratory (computing) support and supplied ideas. DR provided laboratory (experimental) support, supplied ideas, and coordinated the experimental aspects of the work. All authors contributed in drafting the manuscript.
- 1. Adams JR, Schmidtmann ET, Azad AF (1990) Infection of colonized cat fleas, Ctenocephalides felis (Bouche), with a Rickettsia-like microorganism. Am J Trop Med Hyg 43: 400–409.
- 2. Azad AF, Sacci JB, Nelson WM, Dasch GA, Schmidtmann ET (1992) Genetic characterization and transovarial transmission of a typhus-like Rickettsia found in cat fleas. Proc Natl Acad Sci U S A 89: 43–46.
- 3. Raoult D, La Scola B, Enea M, Fournier PE, Roux V (2001) A flea-associated Rickettsia pathogenic for humans. Emerg Infect Dis 7: 73–81.
- 4. Schriefer ME, Sacci JB, Dumler JS, Bullen MG, Azad AF (1994) Identification of a novel rickettsial infection in a patient diagnosed with murine typhus. J Clin Microbiol 32: 949–954.
- 5. Rolain JM, Franc M, Davoust B, Raoult D (2003) Molecular detection of Bartonella quintana B. koehlerae B. henselae B. clarridgeiae Rickettsia felis and Wolbachia pipientis in cat fleas, France. Emerg Infect Dis 9: 338–342.
- 6. Andersson SG, Zomorodipour A, Andersson JO, Sicheritz-Ponten T, Alsmark UC (1998) The genome sequence of Rickettsia prowazekii and the origin of mitochondria. Nature 396: 133–140.
- 7. McLeod MP, Qin X, Karpathy SE, Gioia J, Highlander SK (2004) Complete genome sequence of Rickettsia typhi and comparison with sequences of other rickettsiae. J Bacteriol 186: 5842–5855.
- 8. Ogata H, Audic S, Renesto-Audiffren P, Fournier PE, Barbe V (2001) Mechanisms of evolution in Rickettsia conorii and R. prowazekii. Science 293: 2093–2098.
- 9. Malek JA, Wierzbowski JM, Tao W, Bosak SA, Saranga DJ (2004) Protein interaction mapping on a functional shotgun sequence of Rickettsia sibirica. Nucleic Acids Res 32: 1059–1064.
- 10. Alt-Morbe J, Stryker JL, Fuqua C, Li PL, Farrand SK (1996) The conjugal transfer system of Agrobacterium tumefaciens octopine-type Ti plasmids is closely related to the transfer system of an IncP plasmid and distantly related to Ti plasmid vir genes. J Bacteriol 178: 4248–4257.
- 11. Beranek A, Zettl M, Lorenzoni K, Schauer A, Manhart M (2004) Thirty-eight C-terminal amino acids of the coupling protein TraD of the F-like conjugative resistance plasmid R1 are required and sufficient to confer binding to the substrate selector protein TraM. J Bacteriol 186: 6999–7006.
- 12. Frost LS, Ippen-Ihler K, Skurray RA (1994) Analysis of the sequence and gene products of the transfer region of the F sex factor. Microbiol Rev 58: 162–210.
- 13. Cascales E, Christie PJ (2003) The versatile bacterial type IV secretion systems. Nat Rev Microbiol 1: 137–149.
- 14. Wu M, Sun LV, Vamathevan J, Riegler M, Deboy R (2004) Phylogenomics of the reproductive parasite Wolbachia pipientis wMel: A streamlined genome overrun by mobile genetic elements. PLoS Biol 2: e69. doi: 10.1371/journal.pbio.0020069.
- 15. Horn M, Collingro A, Schmitz-Esser S, Beier CL, Purkhold U (2004) Illuminating the evolutionary history of chlamydiae. Science 304: 728–730.
- 16. Ogata H, Audic S, Barbe V, Artiguenave F, Fournier PE (2000) Selfish DNA in protein-coding genes of Rickettsia. Science 290: 347–350.
- 17. Raoult D, Roux V (1997) Rickettsioses as paradigms of new or emerging infectious diseases. Clin Microbiol Rev 10: 694–719.
- 18. Uchiyama T (2003) Adherence to and invasion of Vero cells by recombinant Escherichia coli expressing the outer membrane protein rOmpB of Rickettsia japonica. Ann N Y Acad Sci 990: 585–590.
- 19. Roux V, Raoult D (2000) Phylogenetic analysis of members of the genus Rickettsia using the gene encoding the outer-membrane protein rOmpB (ompB). Int J Syst Evol Microbiol 50: 1449–1455.
- 20. Fang R, Raoult D (2003) Antigenic classification of Rickettsia felis by using monoclonal and polyclonal antibodies. Clin Diagn Lab Immunol 10: 221–228.
- 21. Rovery C, Renesto P, Crapoulet N, Matsumoto K, Parola P (2005) Transcriptional response of Rickettsia conorii exposed to temperature variation and stress starvation. Res Microbiol 156: 211–218.
- 22. Hogg T, Mechold U, Malke H, Cashel M, Hilgenfeld R (2004) Conformational antagonism between opposing active sites in a bifunctional RelA/SpoT homolog modulates (p)ppGpp metabolism during the stringent response [corrected]. Cell 117: 57–68.
- 23. Andersson JO, Andersson SG (2001) Pseudogenes, junk DNA, and the dynamics of Rickettsia genomes. Mol Biol Evol 18: 829–839.
- 24. Zhang YX, Li J, Guo XK, Wu C, Bi B (2004) Characterization of a novel toxin-antitoxin module, VapBC, encoded by Leptospira interrogans chromosome. Cell Res 14: 208–216.
- 25. Pandey DP, Gerdes K (2005) Toxin-antitoxin loci are highly abundant in free-living but lost from host-associated prokaryotes. Nucleic Acids Res 33: 966–976.
- 26. Gerdes K (2000) Toxin-antitoxin modules may regulate synthesis of macromolecules during nutritional stress. J Bacteriol 182: 561–572.
- 27. Engelberg-Kulka H, Glaser G (1999) Addiction modules and programmed cell death and antideath in bacterial cultures. Annu Rev Microbiol 53: 43–70.
- 28. Mosavi LK, Minor DL, Peng ZY (2002) Consensus-derived structural determinants of the ankyrin repeat motif. Proc Natl Acad Sci U S A 99: 16029–16034.
- 29. Caturegli P, Asanovich KM, Walls JJ, Bakken JS, Madigan JE (2000) AnkA: An Ehrlichia phagocytophila group gene encoding a cytoplasmic protein antigen with ankyrin repeats. Infect Immun 68: 5277–5283.
- 30. Gough J, Karplus K, Hughey R, Chothia C (2001) Assignment of homology to genome sequences using a library of hidden Markov models that represent all proteins of known structure. J Mol Biol 313: 903–919.
- 31. Cazalet C, Rusniok C, Bruggemann H, Zidane N, Magnier A (2004) Evidence in the Legionella pneumophila genome for exploitation of host cell functions and high genome plasticity. Nat Genet 36: 1165–1173.
- 32. Raoult D, Audic S, Robert C, Abergel C, Renesto P (2004) The 1.2-megabase genome sequence of Mimivirus. Science 306: 1344–1350.
- 33. Blatch GL, Lassle M (1999) The tetratricopeptide repeat: A structural motif mediating protein–protein interactions. Bioessays 21: 932–939.
- 34. Chung S, Mondon P, Chang YC, Kwon-Chung KJ (2003) Cryptococcus neoformans with a mutation in the tetratricopeptide repeat-containing gene, CCN1, causes subcutaneous lesions but fails to cause systemic infection. Infect Immun 71: 1988–1994.
- 35. Matsushita O, Okabe A (2001) Clostridial hydrolytic enzymes degrading extracellular components. Toxicon 39: 1769–1780.
- 36. Silverman DJ, Santucci LA, Meyers N, Sekeyova Z (1992) Penetration of host cells by Rickettsia rickettsii appears to be mediated by a phospholipase of rickettsial origin. Infect Immun 60: 2733–2740.
- 37. Connell TD, Metzger DJ, Lynch J, Folster JP (1998) Endochitinase is transported to the extracellular milieu by the eps-encoded general secretory pathway of Vibrio cholerae. J Bacteriol 180: 5591–5600.
- 38. Koonin EV, Aravind L (2000) The NACHT family—A new group of predicted NTPases implicated in apoptosis and MHC transcription activation. Trends Biochem Sci 25: 223–224.
- 39. Erlandsen H, Canaves JM, Elsliger MA, von Delft F, Brinen LS (2004) Crystal structure of an HEPN domain protein (TM0613) from Thermotoga maritima at 1.75 A resolution. Proteins 54: 806–809.
- 40. Gouin E, Egile C, Dehoux P, Villiers V, Adams J (2004) The RickA protein of Rickettsia conorii activates the Arp2/3 complex. Nature 427: 457–461.
- 41. Gil H, Benach JL, Thanassi DG (2004) Presence of pili on the surface of Francisella tularensis. Infect Immun 72: 3042–3047.
- 42. Larsson P, Oyston PC, Chain P, Chu MC, Duffield M (2005) The complete genome sequence of Francisella tularensis, the causative agent of tularemia. Nat Genet 37: 153–159.
- 43. Greub G, Collyn F, Guy L, Roten CA (2004) A genomic island present along the bacterial chromosome of the parachlamydiaceae UWE25, an obligate amoebal endosymbiont, encodes a potentially functional F-like conjugative DNA transfer system. BMC Microbiol 4: 48.
- 44. Qin A, Tucker AM, Hines A, Wood DO (2004) Transposon mutagenesis of the obligate intracellular pathogen Rickettsia prowazekii. Appl Environ Microbiol 70: 2816–2822.
- 45. Collins NE, Liebenberg J, de Villiers EP, Brayton KA, Louw E (2005) The genome of the heartwater agent Ehrlichia ruminantium contains multiple tandem repeats of actively variable copy number. Proc Natl Acad Sci U S A 102: 838–843.
- 46. Brayton KA, Kappmeyer LS, Herndon DR, Dark MJ, Tibbals DL (2005) Complete genome sequencing of Anaplasma marginale reveals that the surface is skewed to two superfamilies of outer membrane proteins. Proc Natl Acad Sci U S A 102: 844–849.
- 47. Alsmark CM, Frank AC, Karlberg EO, Legault BA, Ardell DH (2004) The louse-borne human pathogen Bartonella quintana is a genomic derivative of the zoonotic agent Bartonella henselae. Proc Natl Acad Sci U S A 101: 9716–9721.
- 48. Chain PS, Carniel E, Larimer FW, Lamerdin J, Stoutland PO (2004) Insights into the evolution of Yersinia pestis through whole-genome comparison with Yersinia pseudotuberculosis. Proc Natl Acad Sci U S A 101: 13826–13831.
- 49. Raoult D, Ogata H, Audic S, Robert C, Suhre K (2003) Tropheryma whipplei twist: A human pathogenic actinobacteria with a reduced genome. Genome Res 13: 1800–1809.
- 50. Bentley SD, Maiwald M, Murphy LD, Pallen MJ, Yeats CA (2003) Sequencing and analysis of the genome of the Whipple's disease bacterium Tropheryma whipplei. Lancet 361: 637–644.
- 51. Ewing B, Hillier L, Wendl MC, Green P (1998) Base-calling of automated sequencer traces using phred. I. Accuracy assessment. Genome Res 8: 175–185.
- 52. Audic S, Claverie JM (1998) Self-identification of protein-coding regions in microbial genomes. Proc Natl Acad Sci U S A 95: 10026–10031.
- 53. Lowe TM, Eddy SR (1997) tRNAscan-SE: A program for improved detection of transfer RNA genes in genomic sequence. Nucleic Acids Res 25: 955–964.
- 54. Altschul SF, Madden TL, Schaffer AA, Zhang J, Zhang Z (1997) Gapped BLAST and PSI-BLAST: A new generation of protein database search programs. Nucleic Acids Res 25: 3389–3402.
- 55. Apweiler R, Bairoch A, Wu CH, Barker WC, Boeckmann B (2004) UniProt: The Universal Protein knowledgebase. Nucleic Acids Res 32: D115–D119.
- 56. Marchler-Bauer A, Anderson JB, Cherukuri PF, DeWeese-Scott C, Geer LY (2005) CDD: A Conserved Domain Database for protein classification. Nucleic Acids Res 33: D192–D196.
- 57. Ponting CP, Schultz J, Milpetz F, Bork P (1999) SMART: Identification and annotation of domains from signalling and extracellular protein sequences. Nucleic Acids Res 27: 229–232.
- 58. Volfovsky N, Haas BJ, Salzberg SL (2001) A clustering method for repeat analysis in DNA sequences. Genome Biol 2: RESEARCH0027.
- 59. Eddy SR (1996) Hidden Markov models. Curr Opin Struct Biol 6: 361–365.
- 60. Ogata H, Audic S, Abergel C, Fournier PE, Claverie JM (2002) Protein coding palindromes are a unique but recurrent feature in Rickettsia. Genome Res 12: 808–816.
- 61. Notredame C, Higgins DG, Heringa J (2000) T-Coffee: A novel method for fast and accurate multiple sequence alignment. J Mol Biol 302: 205–217.
- 62. Kumar S, Tamura K, Jakobsen IB, Nei M (2001) MEGA2: Molecular Evolutionary Genetics Analysis software. Bioinformatics 17: 1244–1245.
- 63. Nakamura Y, Itoh T, Matsuda H, Gojobori T (2004) Biased biological functions of horizontally transferred genes in prokaryotic genomes. Nat Genet 36: 760–766.
- 64. Lawrence JG, Ochman H (1998) Molecular archaeology of the Escherichia coli genome. Proc Natl Acad Sci U S A 95: 9413–9417.
- 65. Moret BM, Wyman S, Bader DA, Warnow T, Yan M (2001) A new implementation and detailed study of breakpoint analysis. Pac Symp Biocomput 2001: 583–594.