The hindguts of wood-feeding termites typically contain hundreds of microbial species. Together with their insect host, these gut microbes degrade lignocellulose into usable catabolites. Although past research revealed many facets of the stepwise flow of metabolites in this scheme, not much is known about the breadth of interactions occurring between termite-gut microbes. Most of these microbes are thought to depend on, and to have co-speciated with, their host and each other for millions of years. In this study, we explored the interactions of two spirochetes previously isolated from the very same termite species. As hydrogen (H2) is the central free intermediate in termite-gut lignocellulose digestion, we focused on interactions between two closely related termite-gut spirochetes possessing complementary H2 physiologies: one produces H2, while the other consumes it. In vitro, these two Treponema species markedly enhanced each other's growth. RNA sequencing resolved the transcriptomes of these two closely related organisms, revealing that co-cultivation causes comprehensive changes in global gene expression. The expression of well over a 100 genes in each species was changed >twofold, with over a dozen changed >10-fold. Several changes implicating synergistic cross-feeding of known metabolites were validated in vitro. Additionally, certain activities beneficial to the host were preferentially expressed during consortial growth. However, the majority of changes in gene expression are not yet understandable, but indicate a broad, comprehensive and mutualistic interaction between these closely related, co-resident gut symbionts. The results suggest that staggeringly intricate networks of metabolic and gene interactions drive lignocellulose degradation and co-evolution of termite gut microbiota.
A bacterium's capacity to perform physiological tasks in isolation is not necessarily predictive of how it performs in the natural environment. Take for example the classic model bacterium, Escherichia coli, a versatile organism that degrades many substrates under many growth conditions in pure culture (Boone et al., 2001). In environmental context, much less is known about its physiology (Chang et al., 2004). E. coli probably degrades only a few substrates in situ, because it is outnumbered and likely outprocessed by a diversity of other specialists. Likewise, some species do not express certain traits when grown alone, and what appears to be a cryptic activity only blooms when growth occurs in the presence of other species (Straight et al., 2007). Lastly, host-associated organisms may respond to cues from their host, and in response catalyze activities that impact the host (Palmer et al., 2007). Neither of these activities are typically recapitulated during standard cultivation regimes.
Physiological analyses of model organisms, like E. coli above, have greatly benefited from high-throughput tools, especially microarrays (Chang et al., 2004). However, arrays require extensive design and ground-truthing before even the first experiment can be performed. These constraints are significant, considering that the number of candidate organisms for expression studies has exploded in this era of genome sequencing. Moreover, any successful interpretation of array data becomes complicated when investigating global gene expression of closely related species (sharing high nucleic acid similarities) grown in either defined co-cultures or their natural habitats. The probe-binding nature of the microarray approach is not well suited to distinguish between conserved nucleotide sequences. Thus, array-based studies on co-cultures and communities are essentially limited to examples involving species having very different genomes (Saleh-Lakha et al., 2005).
Breakthroughs in next-generation sequencing not only allow the comparison of expression from highly similar sequences, but also dramatically expedite the pace at which data can be gathered from less-well-studied microbes (Holt et al., 2008; Yoder-Himes et al., 2009) and complex biological environments (Gilbert et al., 2008; Urich et al., 2008). Although transcriptomic calculations are now possible, studies of co-cultures and intact environments are challenging, as they entail inherent difficulties when making comparisons and contrasts. For one, it is very difficult to directly compare the gene expression patterns of cultures when the growth conditions are very dissimilar, and this is the case when environmentally reliant symbionts are removed from their environment—or even one from another in defined co-culture. Furthermore, common RNA-seq techniques do not differentiate the direction in which a transcript is oriented, and there appears to be times when anti-coding RNAs are present, which may not be fully accounted for by many studies (Dornenburg et al., 2010). However, studies of transcriptional output in different conditions do allow one to analyze the impact of individual microbes at a particular point of time, and to produce testable hypotheses about the functions of different members of a microbial community, issues at the crux of molecular microbial ecology.
In this study, we combined the use of classic microbiological cultivation techniques with next-generation sequencing to explore gene expression patterns underlying the metabolic interactions between closely related bacteria that had been isolated from the same microliter-in-scale termite hindgut environment.
The gut communities of wood-feeding termites ferment the polysaccharide fractions of lignocellulose, ultimately providing the termite with compounds such as carbon and energy substrate acetate, amino acids and other essential growth factors (Odelson and Breznak, 1983; Brauman et al., 1992; Abe et al., 2000). During the course of lignocellulose fermentation, the free intermediate hydrogen (H2) is produced and accumulates to concentrations near saturation (Pester and Brune, 2007), before being consumed by homoacetogenic gut bacteria and methanogenic archaea (Breznak and Switzer, 1986; Brauman et al., 1992). It has been estimated that H2+CO2 acetogenic bacteria supply their termite host with up to a third of its acetate supply (Breznak and Switzer, 1986). Together, the fermentation and CO2-reductive acetogenesis-derived acetate can contribute up to 70–100% of the termite host's energy requirements (Drake, 1994).
In this study, we have sought to reveal possible interactions occurring between two previously isolated termite-gut treponemes: Treponema primitia ZAS-2 and Treponema azotonutricium ZAS-9. These two species reside in close proximity in the hindgut of the dampwood termite Zootermopsis angusticolis (Graber et al., 2004), wherein (as in most termites) a diversity of spirochetes constitute a large portion of the total gut microbiota (Breznak, 2002). Previous studies suggest that these bacteria have separate physiological roles in the complex mutualism (Leadbetter et al., 1999; Lilburn et al., 2001; Graber and Breznak, 2004; Graber et al., 2004). However, to what extent they interact with and impact each other and other gut species is less well examined. Certainly, T. primitia is known to depend on an essential growth factor, folate, derived from other gut microbiota (Graber and Breznak, 2005). T. azotonutricium fixes nitrogen (Lilburn et al., 2001) and produces H2 as a fermentation product (Graber et al., 2004), whereas T. primitia is an H2-consuming CO2-reducing homoacetogen (Leadbetter et al., 1999). Their complementary H2 physiologies and their close proximity to each other in the small termite-gut environment begs the question of whether they might engage in other interactions. The genomes of T. azotonutricium and T. primitia are relatively large (3.86 Mb and 4.06 Mb, respectively (Graber et al., 2004) compared with other sequenced treponemes (T. denticola 2.84 Mb (Seshadri et al., 2004); T. pallidum 1.14 Mb (Fraser et al., 1998)). We sought to identify genes that may be relevant to interspecies interactions by analyzing global gene expression during consortial growth of the two, via Illumina transcript-sequencing technology (Illumina, San Diego, CA, USA).
Materials and methods
Bacterial strains and culture media
T. primitia (ZAS-2) and T. azotonutricium (ZAS-9) cultures were grown in 4-YACo media (4% yeast autolysate) supplemented with 20 mM maltose and 80% H2 and 20% CO2 in the headspace. Cultures were grown in 5 ml volumes in 25-ml Balch tubes, with crimp top stoppers in the dark at room temperature. Vitamin, amino-acid and cofactor preparations used to supplement media were as follows:
Vitamin B7: 0.3–0.5 μg biotin (Sigma Aldrich, St Louis, MO, USA) was added per culture tube.
Vitamin B6: 120–200 μg pyridoxal-HCl and pyridoxal-phosphate (Sigma Aldrich) were added per culture tube.
B12 and corrinoids: 30–50 μg of one of the following: (1) hydroxocobalamin acetate salt, (2) hydroxocobalamin hydrochloride, (3) methylcobalamin and (4) cyanocobalamin (Sigma Aldrich), was added per culture tube.
Tryptophan: 60–100 μg tryptophan (Sigma Aldrich) was added per culture tube.
RNA isolation and processing
Total RNA was isolated from two biological replicates per growth condition. Procedures for sample preparation followed from the standard Illumina protocol for RNA-Seq sample preparation available from the manufacturer (Illumina). In short, RNA was isolated using RNeasy kit (Qiagen, Valencia, CA, USA) as per the manufacturer's protocol. Samples were run through the RNeasy procedure twice, with the optional DNase treatment performed in both instances. Total RNA was fragmented using the Ambion RNA fragmentation kit (Ambion, Austin, TX, USA) and protocol. First-strand complementary DNA was prepared following the SuperScript II method (Invitrogen, Carlsbad, CA, USA), using the Invitrogen hexamer random primers to ensure low primer bias. Second-strand complementary DNA was subsequently synthesized by adding to the first-strand reaction second-strand buffer (500 mM Tris-HCl pH 7.8, 50 mM MgCl2, 10 mM dithiothreitol), deoxyribonucleotide triphosphate (0.3 mm), RNaseH (2 U μl−1; Invitrogen #18021-014), Invitrogen hexamer primers and DNA polymerase I (Invitrogen). The final reaction volume for second-strand synthesis was 100μl, and reactions were carried out at 16 °C for 2.5 h.
Complementary DNA sequencing
Fragmented second-strand complementary DNA samples were submitted to the Caltech Sequencing Core facility (Pasadena, CA, USA). Libraries were sequenced as 37-mers using the standard Solexa (Illumina) protocol and pipeline. Sequencing depth information is summarized in Supplementary Table 3.
RNA-Seq data analysis
Illumina raw data provided by the GERALD (Illumina) software package were aligned to a FASTA file containing both T. azotonutricium (ZAS-9) and T. primitia (ZAS-2) genomes using the Maq short read aligning program (Wellcome Trust Sanger Institute, Hinxton, UK). For initial analysis of mapping quality (see Table 1), zero or one misses were allowed per read. All subsequent samples were analyzed with a maximum of one mismatch allowed.
Reads from biological replicates were first compared with each other (a) graphically after mapping onto the two genomes, and then (b) by looking for differences in fold regulation when compared in all pairwise combinations of other replicates of interest. Biological replicates broadly were far more similar to each other than to other samples. Reads from biological replicates were merged and averaged for all further analysis.
To exclude reads that may align ambiguously (that is, to either genome), we assembled hypothetical databases of all possible 37′-mer sequences for each genome, and mapped them to the opposing genome with one mismatch allowed. Additionally, a database of pooled Illumina sequencing data from each pure culture was also aligned to the opposing genome. Reads that ambiguously mapped were excluded from transcriptional analysis. Gene expression values were determined by normalizing the number of reads mapped to a particular gene (excluding ambiguous regions) divided by the size of the gene (also excluding ambiguous regions). The resulting value is the normalized reads per kilobase, in a manner consistent with the gene expression index calculations of previously published reports (Yoder-Himes et al., 2009). In order to adjust for intensity between samples, the ribosomal signal from each sample was used as a standard, and each sample's intensity was multiplied by a factor that would yield an equal ribosomal RNA (rRNA) signal.
In considering up- or downregulated genes, a cutoff of twofold increase in transcription was used. Additionally, except in the case of functional groups and gene clusters used to generate Supplementary Table 1, only genes with greater than 50 adjusted hits per kb of coding DNA were considered in analyses.
Signal intensities were visualized graphically by converting Maq-aligned reads into a .BAR file using the Cisgenome software, and viewed on the Cisgenome browser (Stanford University, Stanford, CA, USA) (Ji et al., 2008).
Quantitative RT-PCR of several T. azotonutricium genes:
clpX (TREAZ# 737).
Endo-1,4-beta-xylanase A precursor (TREAZ# 2717).
Endo-1,4-beta-xylanase A precursor (TREAZ#2718).
Glycoprotein gp2, Endo-1,4-beta-xylanase A precursor (TREAZ#2716).
These qRT measurements reveal expression ratios similar to those reported by RNA-Seq.
In all, 100 μl samples from bacterial cultures were taken daily. Samples were centrifuged at 13 000 g for 5 min, aspirated, resuspended in an equal volume of dH2O, and frozen for later use. Quantitative PCR on bacterial samples followed, using primers specific for the clpX gene of either T. primitia or T. azotonutricium. Quantitative PCR primers of 20 bp length were designed, with the following sequences:
T. azotonutricium clpX (fwd): 5′-IndexTermGGAACTTTTCGATGCTCTGC-3′
T. azotonutricium clpX (rev): 5′-IndexTermGCGCTTAAGGTCTTCCCTCT-3′
T. primitia clpX (fwd): 5′-IndexTermCTCCCGTTTCATTTCTTCCA-3′
T. primitia clpX (rev): 5′-IndexTermGAAATGTTAGACGCCCTCCA-3′
Primers were designed to have a roughly equal amplification product length to avoid large differences in fluorescence intensities. Each pair of primers was tested for melting temperature, specificity and amplification efficiency, and was found to be specific and suitable for q-PCR (each having an E factor greater than 1.75). Quantitative PCR reactions were performed with the iTaq SYBR Green PCR kit and a DNA engine chromo-4 qPCR instrument (Bio-Rad, Hercules, CA, USA). A standard curve of known dilutions of T. primitia and T. azotonutricium genomic DNA was performed with each set of experiments. Triplicate q-PCR reactions were used for each data point. To obtain genomic cell equivalent units, the ribosomal copy number was obtained from the standard curve calculations, and divided by 2 to account for the number of 16S copies in each genome.
Results and discussion
Full and accurate analysis of transcript pools from two closely related organisms grown together relies on the ability to distinguish between highly homologous sequences. Therefore, before analyzing the experimental data, we determined the frequency of cross-identification between the two treponemes used in this study. To do this, a data set of all possible short nucleotide sequences (37 bp, the exact length of the reads) from each genome was generated in silico and aligned to the genome of the other species (Materials and methods). The results (Table 1) demonstrate that only a small number of all possible 37-bp sequences (6518, ca. 0.15%) are identical in both bacteria. A large percentage of these, ca. 45%, are r16S and r23S RNAs, whereas greater than 97% of all non-rRNA genes are completely unique (that is, do not contain a single sequence read having an exact match to the other genome). Relaxing the stringency to allow one mismatch per 37-bp sequence does not yield dramatically less favorable results, with over 92% of the genes being completely unique. Moreover, in no case was a single gene in either genome fully masked; all genes in both organisms had at least one unique 37-bp identifier. This resolution allows complete transcript discrimination and genome-wide analysis in co-culture experiments.
Experimental considerations compelled us to analyze the background noise expected in actual data. To this end, a database totaling nearly 11 million RNA-Seq reads from T. azotonutricium was mapped to the combined genomes of both bacteria. As predicted, the majority of reads (9 million; 82.5%) aligned to T. azotonutricium, and practically all (over 99.9%) of the reads that did map to T. primitia were rRNA (Table 1) This result was expected, as ribosomal transcription typically comprises over 90% of the total transcript pool (Neidhardt and Curtiss, 1996), and rRNAs are typically the most conserved sequences between the genomes (the small subunit rRNA has 93% nucleotide similarity; (Graber et al., 2004)). When all rRNA sequences, except highly variable regions and sequences with up to one mismatch similarity, were masked from the analysis, only 646 reads from one species mapped to the other genome. This led us to conclude that this method was effective at discriminating the signals from two similar genomes. The reciprocal analyses yielded similar trends, and are presented in Table 1.
For gene expression profiling, bacterial cultures of T. primitia, T. azotonutricium and their co-culture were grown on 4YACo medium supplemented with H2 and maltose (Graber et al., 2004). The growth kinetics of each species was followed as a function of genome copy number, that is, using qPCR of unique chromosomal DNA markers from each genome. These measurements reveal that initially each species grew at similar rates, whether in pure or co-culture (shaded region, Figure 1). However, after this initial growth phase, the growth of each species was markedly stimulated in both rate and yield in co-cultures, relative to growth in monoculture. The greater effect was observed for T. azotonutricium (Figure 1). Importantly, although these two species might compete for anabolic nutrients in the medium's yeast autolysate base, at no point were the two species observed to have any negative impact on each other's growth. All samples for gene expression analysis were collected during a period within the later, synergism-dominated growth phase (OD600≈0.35) (Figure 1). Overall, a large set of genes, consisting of approximately 7% of all T. azotonutricium and 4.5% of all T. primitia-coding regions, were differentially regulated as a function of co-cultivation (Supplementary Table 2). In agreement with growth measurements, several genes related to cell division and other aspects of growth are upregulated in co-cultures (Supplementary Table 2). The observation that in the later growth phase co-cultures maintain near-log phase growth rates (while the pure cultures are nearing or entering stationary phase) can also be used to explain the differences between transcript pools in the co-cultures. This is especially true for T. azotonutricium, for which samples were taken in a late stage to allow for sufficient cell growth.
The positive co-culture growth effect on T. primitia might be anticipated when considering the H2 physiologies of the two species. Fermenting gut microbes, including T. azotonutricium, provide homoacetogens like T. primitia a source of H2 (Pester and Brune, 2007). In the culture media, an initial amount of H2 gas (80%), which roughly mimics physiological conditions within the gut, was supplied in the headspace but was not replenished during growth. Previously, the growth of T. primitia has been observed to be noticeably restricted if H2 is not initially supplied in the medium (Graber and Breznak, 2004). Thus, one predicted aspect of synergy between the two strains is the continued production of H2 by T. azotonutricium, as this gas is consumed by T. primitia. Indeed, T. primitia genes associated with H2 utilization were differentially regulated in co-cultivation: among the most highly upregulated T. primitia genes were those that encoded several hydrogenase-like proteins; in turn, the genes for several other hydrogenase-like proteins are markedly downregulated during co-cultivation (Table 2, Supplementary Table 1). These findings are consistent with previously published reports of hydrogenase expression in methanogenic H2 consumers (Desulfovibrio vulgaris), when cultured together with a hydrogen producer (Walker et al., 2009).
When the two treponemes were co-cultured, an additional effect on T. primitia genes associated with CO2-reductive acetogenesis was observed. In pure culture, both a selenocysteine-containing (fdhFsec) and a non-selenocysteine (fdhFcys) variant of the enzyme formate dehydrogenase, which catalyzes an early step of the Wood–Ljungdahl pathway, were transcribed (Matson et al., 2010). During growth in co-cultures, the selenocysteine form of the enzyme was upregulated, whereas the non-selenium form was downregulated (Table 2, Supplementary Tables 1 and 4).
Co-cultivation with T. primitia significantly enhanced the growth rate and yield of T. azotonutricium (Figure 1). Examination of the gene expression data and the genome sequences of the two treponemes suggested several potential growth factors that might be involved in the interaction. The differential regulation of many genes involved in corrinoid production or transport, vitamin B7 (biotin), vitamin B6 (pyridoxal phosphate) and coenzyme-A (Table 2, Supplementary Table 1), was observed. In the case of vitamin B7, several relevant regulatory or transport genes are downregulated when T. azotonutricium is co-cultivated with T. primitia (Table 2, Supplementary Table 1), but only the latter has a complement of the genes to synthesize B7 (Supplementary Figure 1). Similarly, an important gene for the synthesis of vitamin B6 precursors (for example, phosphoserine aminotransferase) (Lam and Winkler, 1990) and several genes that require vitamin B6 for full activity were also downregulated during consortial growth of T. azotonutricium (Table 2, Supplementary Table 1). The enzyme responsible for producing the active form of vitamin B6 (pyridoxal kinase) is exclusive to the genome of T. primitia (Supplementary Figure 1). Finally, key genes for coenzyme-A biosynthesis are absent in T. azotonutricium but present in T. primitia (Supplementary Figure 1).
One explanation for the upregulation of genes that transport vitamin B7 or require vitamin B6 for activity is that as the bacterial population size increases, the amount of available vitamins is increasingly scarce, and thus bacteria are more reliant on importing and using what little vitamins are present.
To examine if any of these candidate growth factors might be relevant to the observed synergistic growth of the species during their co-culture, the growth medium of T. azotonutricium pure cultures was supplemented. The results (Figure 2) demonstrate that vitamin B6, and to a lesser extent B7 and coenzyme-A, have a positive impact on growth. None of the corrinoid or B12 preparations tested improved the growth of T. azotonutricium, nor were the additions of any of these supplements observed to have any beneficial effect on the growth of T. primitia.
In addition to the candidate cofactors and vitamins that were identified and explored above, we note that a number of hypothetical genes are also regulated differently in co-culture (Figure 3, Supplementary Table 2). The large number of these genes suggests that additional processes may be involved in complex mutualistic symbiosis. The abundance of genes regulated by these conditions also serves to underscore the large effects that growth in the presence of other microbes has on the physiology and behavior of another bacterial species. Looking ahead, it is possible that the accumulation of expression studies of microbial communities can be used to highlight uncharacterized genes that act as putative symbiosis determinants.
A hallmark of several insect–microbe symbioses is the bacterial production of factors vital to the host, including vitamins, cofactors and essential amino acids (reviewed in Moran, 2006). Vitamins B6 and B7, the production of which appears to aid in the growth of T. azotonutricium when it is grown in co-culture with T. primitia, have a role in the symbiosis between tse-tse flies and their endosymbiont Wigglesworthia glossinidia brevipalpis (Akman et al., 2002). Genes for several amino-acid biosynthesis pathways were upregulated during the consortial growth of the two treponemes, including those for aromatic amino acids and methionine biosyntheses in T. primitia, and for branched-chain amino acids in T. azotonutricium (Table 2). Together these represent six out of ten amino acids known to be essential in insects (Gil et al., 2003). Curiously, the tryptophan synthesis pathway appears to be absent in the diazotroph T. azotonutricium, but the expression of these genes was highly induced in T. primitia when the two were grown together. Past studies had revealed that T. azotonutricium is capable of growth as a bona-fide N2-fixing bacterium (Lilburn et al., 2001), yet required that the medium be supplemented with yeast autolysate while doing so, presumably at least in part to complement its need for tryptophan. Thus, our results suggest that the fixation of N2, ultimately into a full suite of essential amino acids, is a consortial activity in the N-limited lignocellulose-degrading environment of the termite gut. In the case of the branched-chain amino acids (for which both strains appear to have all required biosynthetic components), co-cultivation stimulates expression of key synthesis genes in T. azotonutricium and key transport genes in T. primitia (Table 2, Supplementary Table 1). Taken together, the gene expression patterns observed during the consortial growth of the two species suggest a streamlined division of biosynthetic labor and shared production of key nutrients.
The upregulation of essential amino-acid biosynthesis genes in co-culture suggests that their production may also benefit the host and other community members, as these essential amino acids are often implicated in insect/bacteria symbioses (Shigenobu et al., 2000; Gil et al., 2003; Nakabachi et al., 2006). The recently published genomes of two endosymbionts of termite-gut protozoa have also suggested the importance of other aspects of amino-acid and vitamin production in the symbiosis (Hongoh et al., 2008a, 2008b).
The genomes of intracellular endosymbionts of insects are often highly reduced (Shigenobu et al., 2000; Akman et al., 2002; Gil et al., 2003; Nakabachi et al., 2006; Hongoh et al., 2008a, 2008b) and underlie the obligate reliance of these bacteria on nutrients and factors supplied by the host. In return, many such endosymbionts act almost exclusively as essential amino acids and vitamin factories, capable of little else (Shigenobu et al., 2000; Akman et al., 2002; Gil et al., 2003; Nakabachi et al., 2006). In contrast, these termite-gut spirochetes are not intracellular residents of their host's tissues, and have comparatively large genomes, suggesting that they are capable of performing many more tasks in their species-rich symbiotic environment than their endosymbiontic counterparts. Several of these tasks, as implicated by expression and activity data from this and previous studies, are presented in Figure 4. They include acetate production during sugar fermentation and CO2-reductive acetogenesis, H2 cycling, nitrogen fixation, amino-acid biosynthesis and vitamin and co-factor production (Leadbetter et al., 1999; Lilburn et al., 2001; Graber et al., 2004). In return, the termite provides its microbiota with finely ground particles of recalcitrat carbon and energy source, lignocellulose and a controlled environment.
In addition to providing insights into the symbiotic interactions of these two treponemes in the context of the termite gut, the RNA-Seq data that were mapped onto the two genomes also provided information on genes and intergenic transcripts that had not yet been predicted. For example, on scanning the two genomes for intergenic loci with high gene expression, we were able to identify seven highly transcribed intergenic regions in the two genomes. Five of these are between previously annotated genes of T. primitia (between gene pairs 175:176, 2323:2324, 2456:2457, 2870:2871 and 3885:3886). The other two intergenic transcripts were in T. azotonutricium (between gene pairs 486:487 and 953:954). The high transcript levels of these genes are displayed in Supplementary Table 4, and are generally higher than those of mRNAs from the predicted, annotated genes. Upon further analysis we were able to predict a putative role for three of these intergenics. All three of these newly annotated genes appear to be ribozymes, with RnaseP genes being found in both genomes and what appears to be tmRNA in the genome of T. primitia. There remains an inherent difficulty in the in-silico identification of genes based on predictions of RNA folding (as opposed to proposing canonical open reading frames after scanning all possible translation reading-frames). Thus, RNA-Seq provides a wet-bench experimental method to aid in the identification of non-canonical open reading frames. Data on the expression of one of these genes, the tmRNA from the genome of T. primitia, are provided in Figure 5a.
Apart from intergenic sequences, we have scrutinized graphical displays of transcripts to identify atypical transcription patterns in the two genomes. An interesting example of an atypical transcript pattern is a gene that had overly abundant transcripts towards the gene center, as opposed to the two ends (Figure 5b). In order to determine which transcripts for this region of the gene were in the coding direction or noncoding (antisense) direction, we used qRT-PCR primers specific for either direction, targeting different areas of the gene. As shown in Figure 5b (and inset), whereas the coding transcripts are relatively constant throughout the gene, a large amount of transcripts in the antisense direction are present toward the gene center. This highly transcribed anti-sense region contains six evenly spaced direct repeats of unknown function, but which may help to explain the periodicity of transcript depth observed in the central portion of the gene. This finding is similar to those detailed in a recent publication that uses a variation of the RNA-seq protocol to compose a genome-wide map of both coding and antisense transcripts (Dornenburg et al., 2010).
This work reveals that, when grown together, two termite-gut Treponema species influence each other's gene expression in a far more comprehensive and nuanced manner than might have been predicted based on the results of previous studies on the respective pure cultures. Although H2-based interactions are predicted by known physiologies, using new techniques we find a division of labor between the bacteria, and uncover unforeseen symbiotic interactions. On the road to understanding the even more complex interactions that occur among the hundreds of microbial species residing in termite and other gut environments, we believe that studies of defined microbial consortia of representative strain isolates become a promising avenue toward gaining a better understanding of such systems. Despite the inherent difficulties in comparing transcript signals from different organisms and co-cultures (as in this study), we expect that deep RNA sequencing will enable and expedite such studies, revealing genes and interactions underlying the associations, and aiding in the development of many new hypotheses and new directions of research.
Abe T, Bignell DE, Higashi M . (2000). Termites: Evolution, Sociality, Symbioses, Ecology. Kluwer Academic Publishers: Dordrecht and Boston.
Akman L, Yamashita A, Watanabe H, Oshima K, Shiba T, Hattori M et al. (2002). Genome sequence of the endocellular obligate symbiont of tsetse flies, Wigglesworthia glossinidia. Nat Genet 32: 402–407.
Boone DR, Castenholz RW, Garrity GM . (2001). Bergey's Manual of Systematic Bacteriology. Garrity GM (ed.), 2nd edn. Springer: New York.
Brauman A, Kane MD, Labat M, Breznak JA . (1992). Genesis of acetate and methane by gut bacteria of nutritionally diverse termites. Science 257: 1384–1387.
Breznak JA, Switzer JM . (1986). Acetate synthesis from H(2) plus CO(2) by termite gut microbes. Appl Environ Microbiol 52: 623–630.
Breznak JA . (2002). Phylogenetic diversity and physiology of termite gut spirochetes. Integr Comp Biol 42: 313–318.
Chang DE, Smalley DJ, Tucker DL, Leatham MP, Norris WE, Stevenson SJ et al. (2004). Carbon nutrition of Escherichia coli in the mouse intestine. Proc Natl Acad Sci USA 101: 7427–7432.
Dornenburg JE, Devita AM, Palumbo MJ, Wade JT . (2010). Widespread antisense transcription in Escherichia coli. MBio 1: e00024-10.
Drake HL . (1994). Acetogenesis. Chapman & Hall: New York.
Fraser CM, Norris SJ, Weinstock GM, White O, Sutton GG, Dodson R et al. (1998). Complete genome sequence of Treponema pallidum, the syphilis spirochete. Science 281: 375–388.
Gil R, Silva FJ, Zientz E, Delmotte F, González-Candelas F, Latorre A et al. (2003). The genome sequence of Blochmannia floridanus: comparative analysis of reduced genomes. Proc Natl Acad Sci USA 100: 9388–9393.
Gilbert JA, Field D, Huang Y, Edwards R, Li W, Gilna P et al. (2008). Detection of large numbers of novel sequences in the metatranscriptomes of complex marine microbial communities. PLoS One 3: e3042.
Graber JR, Breznak JA . (2004). Physiology and nutrition of Treponema primitia, an H2/CO2-acetogenic spirochete from termite hindguts. Appl Environ Microbiol 70: 1307–1314.
Graber JR, Breznak JA . (2005). Folate cross-feeding supports symbiotic homoacetogenic spirochetes. Appl Environ Microbiol 71: 1883–1889.
Graber JR, Leadbetter JR, Breznak JA . (2004). Description of Treponema azotonutricium sp. nov. and Treponema primitia sp. nov., the first spirochetes isolated from termite guts. Appl Environ Microbiol 70: 1315–1320.
Holt KE, Parkhill J, Mazzoni CJ, Roumagnac P, Weill FX, Goodhead I et al. (2008). High-throughput sequencing provides insights into genome variation and evolution in Salmonella Typhi. Nat Genet 40: 987–993.
Hongoh Y, Sharma VK, Prakash T, Noda S, Taylor TD, Kudo T et al. (2008a). Complete genome of the uncultured Termite Group 1 bacteria in a single host protist cell. Proc Natl Acad Sci USA 105: 5555–5560.
Hongoh Y, Sharma VK, Prakash T, Noda S, Toh H, Taylor TD et al. (2008b). Genome of an endosymbiont coupling N2 fixation to cellulolysis within protist cells in termite gut. Science 322: 1108–1109.
Ji H, Jiang H, Ma W, Johnson DS, Myers RM, Wong WH . (2008). An integrated software system for analyzing ChIP-chip and ChIP-seq data. Nat Biotechnol 26: 1293–1300.
Lam HM, Winkler ME . (1990). Metabolic relationships between pyridoxine (vitamin B6) and serine biosynthesis in Escherichia coli K-12. J Bacteriol 172: 6518–6528.
Leadbetter JR, Schmidt TM, Graber JR, Breznak JA . (1999). Acetogenesis from H2 plus CO2 by spirochetes from termite guts. Science 283: 686–689.
Lilburn TG, Kim KS, Ostrom NE, Byzek KR, Leadbetter JR, Breznak JA . (2001). Nitrogen fixation by symbiotic and free-living spirochetes. Science 292: 2495–2498.
Matson EG, Zhang X, Leadbetter JR . (2010). Selenium controls transcription of paralogous formate dehydrogenase genes in the termite gut acetogen, Treponema primitia. Environ Microbiol 12: 2245–2258.
Moran NA . (2006). Symbiosis. Curr Biol 16: R866–R871.
Nakabachi A, Yamashita A, Toh H, Ishikawa H, Dunbar HE, Moran NA et al. (2006). The 160-kilobase genome of the bacterial endosymbiont Carsonella. Science 314: 267.
Neidhardt FC, Curtiss R . (1996). Escherichia coli and Salmonella: Cellular and Molecular Biology, 2nd edn. ASM Press: Washington, DC.
Odelson DA, Breznak JA . (1983). Volatile fatty acid production by the hindgut microbiota of xylophagous termites. Appl Environ Microbiol 45: 1602–1613.
Palmer KL, Aye LM, Whiteley M . (2007). Nutritional cues control Pseudomonas aeruginosa multicellular behavior in cystic fibrosis sputum. J Bacteriol 189: 8079–8087.
Pester M, Brune A . (2007). Hydrogen is the central free intermediate during lignocellulose degradation by termite gut symbionts. ISME J 1: 551–565.
Saleh-Lakha S, Miller M, Campbell RG, Schneider K, Elahimanesh P, Hart MM et al. (2005). Microbial gene expression in soil: methods, applications and challenges. J Microbiol Methods 63: 1–19.
Seshadri R, Myers GS, Tettelin H, Eisen JA, Heidelberg JF, Dodson RJ et al. (2004). Comparison of the genome of the oral pathogen Treponema denticola with other spirochete genomes. Proc Natl Acad Sci USA 101: 5646–5651.
Shigenobu S, Watanabe H, Hattori M, Sakaki Y, Ishikawa H . (2000). Genome sequence of the endocellular bacterial symbiont of aphids Buchnera sp APS. Nature 407: 81–86.
Straight PD, Fischbach MA, Walsh CT, Rudner DZ, Kolter R . (2007). A singular enzymatic megacomplex from Bacillus subtilis. Proc Natl Acad Sci USA 104: 305–310.
Urich T, Lanzén A, Qi J, Huson DH, Schleper C, Schuster SC . (2008). Simultaneous assessment of soil microbial community structure and function through analysis of the meta-transcriptome. PLoS ONE 3: e2527.
Walker CB, Stolyar S, Chivian D, Pinel N, Gabster JA, Dehal PS et al. (2009). Contribution of mobile genetic elements to Desulfovibrio vulgaris genome plasticity. Environ Microbiol 11: 2244–2252.
Yoder-Himes DR, Chain PS, Zhu Y, Wurtzel O, Rubin EM, Tiedje JM et al. (2009). Mapping the Burkholderia cenocepacia niche response via high-throughput sequencing. Proc Natl Acad Sci USA 106: 3976–3981.
We thank our laboratory colleagues and participants in Caltech's GEC facility for their insights and advice. This research was supported by the DOE (DE-FG02-07ER64484) and the NSF (EF-0523267).
The authors declare no conflict of interest.
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Rosenthal, A., Matson, E., Eldar, A. et al. RNA-seq reveals cooperative metabolic interactions between two termite-gut spirochete species in co-culture. ISME J 5, 1133–1142 (2011). https://doi.org/10.1038/ismej.2011.3
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