- Research article
- Open Access
Global mapping of transcription start sites and promoter motifs in the symbiotic α-proteobacterium Sinorhizobium meliloti1021
BMC Genomics volume 14, Article number: 156 (2013)
Sinorhizobium meliloti is a soil-dwelling α-proteobacterium that possesses a large, tripartite genome and engages in a nitrogen fixing symbiosis with its plant hosts. Although much is known about this important model organism, global characterization of genetic regulatory circuits has been hampered by a lack of information about transcription and promoters.
Using an RNAseq approach and RNA populations representing 16 different growth and stress conditions, we comprehensively mapped S. meliloti transcription start sites (TSS). Our work identified 17,001 TSS that we grouped into six categories based on the genomic context of their transcripts: mRNA (4,430 TSS assigned to 2,657 protein-coding genes), leaderless mRNAs (171), putative mRNAs (425), internal sense transcripts (7,650), antisense RNA (3,720), and trans-encoded sRNAs (605). We used this TSS information to identify transcription factor binding sites and putative promoter sequences recognized by seven of the 15 known S. meliloti σ factors σ70, σ54, σH1, σH2, σE1, σE2, and σE9). Altogether, we predicted 2,770 new promoter sequences, including 1,302 located upstream of protein coding genes and 722 located upstream of antisense RNA or trans-encoded sRNA genes. To validate promoter predictions for targets of the general stress response σ factor, RpoE2 (σE2), we identified rpoE2-dependent genes using microarrays and confirmed TSS for a subset of these by 5′ RACE mapping.
By identifying TSS and promoters on a global scale, our work provides a firm foundation for the continued study of S. meliloti gene expression with relation to gene organization, σ factors and other transcription factors, and regulatory RNAs.
Transcription is the first committed step of gene expression in prokaryotes, and as such is highly regulated. Promoter sequences direct the transcription of both coding and non-coding RNAs by acting as target sites for specific RNA polymerase binding and activity [1–3]. Bacteria employ an ingenious machinery to adapt effectively and economically to conditions of stress or environmental changes. The initial mechanism of transcription regulation is based on recruitment of certain sigma (σ) factors by RNA polymerase core enzyme (RNAP). Complex formation with σ factors is essential for RNAP binding to a particular promoter sequence and thus for transcription initiation .
Genome-wide identification of promoter sequences facilitates identification of DNA-binding sites for regulatory proteins and also provides insights into the organization of transcriptional units. RNAseq approaches have allowed the large-scale identification of transcription start sites (TSS) in the ε-proteobacterium Helicobacter pylori and the cyanobacteria Synechocystis sp., Synechococcus elongatus, and Anabaena sp., facilitating the characterization of promoter sequence motifs upstream of the TSS. These approaches revealed an unexpected abundance of cis-encoded antisense RNAs (asRNA) and trans-encoded sRNAs (sRNA), and thereby illuminated a previously unknown dimension of prokaryotic transcriptional activity [4–7]. This picture is consistent with RNAseq studies in diverse Gram-positive and Gram-negative bacteria [8–17].
The α-class of the Proteobacteria comprises diverse bacteria with complex lifestyles, including obligate and facultative plant- and animal-associated bacteria (engaging in both mutualistic and pathogenic interactions), phototrophs, chemoorganotrophs, and chemolithotrophs . In addition, eukaryotic mitochondria are proposed to have arisen from an ancient α-proteobacterium . Despite their importance, little is known about α-proteobacterial transcriptome organization. This study presents the first comprehensive mapping of TSS and assignment of identified promoter sequences to σ factors in an α-proteobacterium. Sinorhizobium meliloti exists either in a free-living life-style in the soil or in symbiosis with a leguminous plant host. In the symbiotic relationship, the bacteria inhabit root nodules, differentiate into polyploid bacteroids, and fix nitrogen to the benefit of the host . Functions for these distinct lifestyles are encoded in the tripartite S. meliloti genome: a single chromosome (3.54 Mbp) and two megaplasmids, pSymA (1.35 Mbp) and pSymB (1.68 Mbp) [20–22].
To adapt to environmental changes or stress situations, S. meliloti can draw on a set of 15 σ factors [20, 23]. RpoD (σ70) provides for housekeeping functions, while alternative σ factors are usually involved in adaptation to specific stresses or growth conditions . RpoN (σ54) is essential for transcription of nitrogen fixation-related genes . Two RpoH σ factors, with sequence similarity to the Escherichia coli heat shock σ32, were identified in S. meliloti; RpoH1 (σH1) was found to be largely responsible for adaptation to heat shock, oxidative stress, and pH changes, whereas the role of RpoH2 (σH2) is largely unknown . At least 11 σ factor genes (rpoE1-rpoE10, fecI) are annotated in the S. meliloti genome as encoding extracytoplasmic function (ECF) σ factors, which are usually regulated by anti-σ factors. The ECF σ factor, RpoE2 (σE2), was characterized as the regulator of at least 44 genes, including rpoH2 and rpoE5, and was inferred to be a global regulator of general stress adaptation and the hyperosmotic stress response [27, 28].
The RNAseq approach reported in this study obtained 17,001 experimentally mapped TSS, including both protein-coding and non-coding transcripts. We were able to predict 2,847 σ factor-specific promoter sequences in appropriate distance to a TSS. This newly defined landscape of TSS and promoter motifs increases our knowledge of promoter properties and will facilitate further analyses of transcriptional and post-transcriptional regulation processes in S. meliloti.
Results and discussion
Global mapping of transcription start sites
To comprehensively map TSS of the S. meliloti 1021 transcriptome, RNA populations derived from 16 different growth and stress conditions were pooled and used for cDNA library preparation (Methods). These conditions included exponential and stationary phase growth in three different media, temperature and pH shifts, oxidative and high salt stress, microoxia, carbon or nitrogen starvation, and exposure to the plant-secreted flavonoid, luteolin. This flavonoid induces expression of bacterial nodulation genes, which are required for the establishment of symbiosis . S. meliloti 1021 carries a mutation in expR encoding a global LuxR-type transcriptional regulator engaged in quorum sensing. This regulator affects multiple processes including exopolysaccharide biosynthesis and motility [30–32]. In order to map ExpR-dependent transcripts, which would otherwise be lacking, RNA from an expR+ derivative of S. meliloti 1021 was also included in our pool. Enzymatic treatment of RNA samples with terminator 5′-phosphate-dependent exonuclease resulted in enrichment of transcripts with primary 5′ ends, prior to cDNA synthesis and deep sequencing (Methods).
Our procedure for mapping and classifying TSS is diagrammed in Additional file 1: Figure S1 and described in detail in Methods. Briefly, 37,792,608 reads were obtained, of which 11,230,166 passed all filtering criteria, and subsequently were subjected to TSS determination and classification. TSS assigned to tRNAs, repeats, and transposons are listed separately (Additional file 2: Table S1).
Overall, 17,001 TSS, not including those listed in Table S1, were grouped into six categories based on their genomic context with respect to a minimal transcription unit (MTU) model (Methods; Figure 1a; Additional file 2: Table S2). TSS representing the prominent 5′ end of a sequence contig overlapping in sense orientation a region of 54 nt upstream of the start codon of protein-coding genes were classified as (i) TSS of mRNAs (mTSS). 54 nt were defined as the minimal region upstream of the ATG to cover promoter motifs and the ribosome binding site, which are more likely to be associated with an mRNA than to a trans-encoded sRNA. (ii) TSS were assigned to leaderless transcripts (lmTSS), if matching the first nucleotide of the translation initiation codon. The class of (iii) putative TSS of mRNAs (pmTSS) comprises TSS that are difficult to distinguish: for any given pmTSS, it is uncertain if the TSS represents an mRNA of a protein-coding gene possessing a long 5′-UTR or a TSS of a trans-encoded sRNA. (iv) Sense TSS (seTSS) represent internal transcripts in the same orientation as, and located within, protein-coding genes. (v) TSS of cis-encoded antisense RNAs (asTSS) are orientated in antisense to protein-coding target genes, and (vi) TSS of trans-encoded sRNAs (sTSS) are located in intergenic regions (IGR) and within a defined distance from neighboring genes. Figures 1b and 1c give an overview of the location and number of TSS in each category, which are discussed in more detail below.
mTSS(TSS associated with mRNAs)
A total of 4,430 mTSS were assigned to 2,657 protein-coding genes (Figures 1b and 1c; Additional file 2: Table S2). The total number of S. meliloti annotated protein- coding genes is 6296 , and 1090 operons were predicted . Assuming a rough estimate of three co-transcribed genes per operon, we have identified TSS for most protein-coding genes in the S. meliloti genome. About 60% (1,644 genes) appear to contain a single TSS, while the remaining genes contain multiple TSS. At least 12 putative TSS were identified for each of the genes SMc01904, SMc02122, and SMc02396 (Additional file 2: Table S2). The most frequent initiating nucleotide for mTSS transcripts was A (47.9%), followed by G (23.6%), T (14.8%), and C (13.7%) (Figure 2a). This agrees with observations that purine nucleotides are the most common initiating nucleotide in bacteria [15, 35], a preference that may be explained by the relatively larger pool size of purine vs. pyrimidine nucleotides .
The existence of alternative promoters for a single gene is one explanation that could account for multiple TSS, as exemplified by pstS, which encodes a phosphate-binding periplasmic protein, and was previously shown to have two TSS located downstream from two PhoB binding motifs (B1 and B2) corresponding to TSS S8 and S9 of Figure 1d . Similarly, ctrA, which encodes a global cell cycle regulator, showed two strongly accumulating transcripts corresponding to TSS S2 and S6 (Figure 1d) that were previously identified downstream from conserved promoter motifs (Figure 1d) . Alternatively, post-transcriptional processing of the 5′-UTR of mRNAs may account for multiple mTSS located downstream of TSS associated with conserved promoter motifs, as is plausible for six TSS of pstS (S1, S3, S4, S5, S8, and S9 in Figure 1d) and four TSS of ctrA (S1, S3, S4, and S5 in Figure 1d).
The average mTSS-to-start-codon distance was ~ 68 nt (Figure 2b), somewhat longer than previously reported for Salmonella enterica serovar Typhimurium and H. pylori. Moreover, the average distance increases to ~80 nt if pmTSS lengths (see below) are included in the calculation. In 40% of all cases, the distance between the mTSS and start codon is between 40 and 100 nt. The maximum distance was 309 nt for the mRNA leader transcript of SMc02724 (Additional file 2: Table S2; ). 5′-UTRs longer than 100 nt were found preceding 1,041 genes (1,466 if pmTSS are also included). This indicates that long 5′-UTRs are not unusual in S. meliloti and may even signify complex mechanisms of gene regulation, as is likely the case for ctrA (Figure 1d; ).
To identify new protein-coding genes that were missed in previous genome annotations [20, 33], we followed the procedure described in Methods and outlined in Additional file 1: Figure S2. This included screening for translational signals, such as ribosome binding sites (RBS) and translational start and stop codons. This approach yielded 221 TSS, associated with 71 new and 150 alternative translational units (Additional file 2: Table S3). To increase the probability of annotating only genuine open reading frames (ORFs), we searched the NCBI nonredundant protein database for orthologs of these newly identified genes. Genes that had orthologs in other α-proteobacteria were named according to the scheme, SMx_ORF_x, and added to the GenDB S. meliloti genome database .
lmTSS(TSS associated with leaderless transcripts)
171 TSS of leaderless transcripts mapped to the first nucleotide of the corresponding start codon (Figures 1a, 1b, and 2b). Only a single TSS was found for 112 of these lmTSS, with the remainder found in combination with mTSS (n=52), pmTSS (n=4), or both (n=3) (Additional file 2: Table S2). Leaderless transcripts were also observed in Synechocystis sp. PCC6803, E. coli, Rhodobacter sphaeroides, and Pseudomonas putida[40–43]. All lmTSS initiate with an AUG triplet, consistent with results in E. coli showing that the 5′-terminal AUG of leaderless mRNAs is important for ribosome recognition and interaction , and that non-AUG start codons are inefficient . Also, a recent study proposed a mechanism for leaderless mRNA translation in E. coli. In this mechanism, the mazEF stress-induced toxin-antitoxin system, in particular the endoribonuclease MazF, plays an important role in maturation of both leaderless mRNAs and a novel, processed 16S rRNA. Assembly of the ribosome with this novel rRNA molecule results in an alternative translational machinery, which is able to translate two classes of leaderless transcripts: those processed via MazF and naturally occurring leaderless mRNAs . In S. meliloti, our observation that most genes with leaderless transcripts possess a single TSS (n=112), suggests that naturally occurring leaderless mRNAs are preferred over processed leaderless transcripts. It is possible that the 59 leaderless mRNAs for which an alternative TSS was identified were processed via endoribonucleases similar to MazF in E. coli, but such a mechanism has not yet been described in S. meliloti.
Organization of protein-coding genes into operons is a common feature in bacterial genomes. Recently, we reported 67 experimentally validated operons and 1,090 predicted operons in the S. meliloti 1021 genome . TSS for 47 of those experimentally validated operons and 613 of the predicted operons were identified in our RNAseq data (Additional file 2: Table S4).
pmTSS(TSS associated with putative mRNAs)
A special situation is illustrated by 425 pmTSS, of which 122 represent the only TSS identified for the corresponding gene (Figure 1b; Additional file 2: Table S2). In many cases, it is unclear if these pmTSS represent mRNAs with unusually long 5′-UTRs or non-coding transcripts. One such example is illustrated by SMc02853, which possesses two pmTSS (Figure 1d). On the other hand, the most distal TSS of ctrA (S6 in Figure 1d) almost certainly represents a transcript with a long 5′-UTR (291 nt), because CtrA was shown to bind upstream of this TSS . CtrA also binds to four additional sites downstream of the S6 TSS suggesting a complex mechanism of autoregulation (Figure 1d; ).
seTSS(TSS associated with internal sense transcripts of ORFs)
Sense TSS must meet two criteria: they must be located in the same orientation as a protein-coding gene and within the corresponding ORF. Sense transcripts are the largest group of TSS in our study: 7,650 were classified as belonging to sense transcripts; and therefore, approximately half of all identified TSS correspond to internal fragments of mRNA transcripts (Figure 1c; Additional file 2: Table S2).
A high proportion of sense transcripts was also observed in RNAseq studies of other prokaryotes, e.g. Synechocystis sp. PCC6803 and Anabaena sp. PCC7120, but the functional role of these RNA fragments, if any, remains to be elucidated [5, 6]. It is possible that sense transcripts may act as target mimicry molecules that sequester sRNAs, asRNAs, or ribonucleases from their respective mRNA target domains . Presumably, a small proportion of sense fragments may represent alternative mRNAs that allow for synthesis of shorter protein isoforms in S. meliloti. However, a more likely explanation is that despite the procedure we used to enrich for transcripts with primary 5′ ends, the majority of sense fragments correspond to abundant processed derivatives of their respective mRNAs rather than independent, primary mRNAs transcribed from their own promoters .
asTSS (TSS of cis-encoded antisense sRNAs)
Cis-encoded antisense RNAs act as regulatory RNA via perfect binding to their corresponding target mRNAs encoded on the opposite DNA strand. The first genome-wide RNAseq-based screen for non-coding transcripts in S. meliloti identified 117 asRNAs . However, antisense RNA detection was limited in that study, because the protocol was designed to preferentially detect short RNAs. This study greatly increased the number of antisense transcripts with the identification of 3,720 asTSS that were assigned to 2957 asRNAs associated with the noncoding strand of protein-coding genes (Figures 1b and 1c; Additional file 2: Table S2). Approximately 35% of the protein-coding genes in S. meliloti (2,210 out of 6,296 genes) had antisense transcripts (Figure 1c; Additional file 2: Table S2). For 1,648 target genes, a single asTSS was identified, while the remaining genes appear to contain two or more asTSS (Figure 1c). An example of an antisense RNA with three TSS, SMb_asRNA_3039, is shown in Figure 1e. Occurrence of numerous antisense transcripts associated with a single protein-coding gene most likely represents processed products of a single, primary non-coding asRNA, rather than transcripts of independent asRNA genes. Examples are SMb21548, SMc02498, and SMc03761 with 50, 14, and 12 asTSS, respectively (Additional file 2: Table S2). The three replicons, chromosome, pSymA, and pSymB represent 54.6%, 20.2%, and 25.2% of the total genome size in bp. Taking into account the different replicon sizes, antisense transcripts were weakly overrepresented on pSymA (23.9%) and pSymB (26.5%) (Figure 1b; Additional file 2: Table S2). The strand-specific location of antisense transcripts on pSymB shows a slight preference for the minus strand, whereas it is virtually equal on the remaining replicons (Figure 1b).
The observed features for cis-encoded antisense sRNAs in S. meliloti are in good agreement with other bacterial transcriptomes. Three studies detected antisense transcription of ~27% to ~50% of the annotated protein-coding genes in two cyanobacteria and H. pylori[4–6]. It is tempting to speculate that antisense transcriptional activity is widespread in prokaryotic genomes. However, antisense transcriptional activity represented less than 5% of the protein-coding genes in Chlamydia trachomatis, Staphylococcus aureus, P. syringae, Vibrio cholerae, and S. enterica[12, 15, 46–48]. It is unknown whether this variation reflects differences in experimental and data analysis procedures or biological mechanisms.
The total length of each transcript in our study is unknown due to the method we used for cDNA library preparation. Prokaryotic asRNAs are generally short transcripts of approximately 100 to 300 nt . This number is in good agreement to the size range (59 to 258 nt) of 117 S. meliloti asRNAs identified in Schlüter et al. . However, several asRNAs of other bacterial species were as long as 7,000 nt [49–53].
Depending on the location of an asRNA relative to its target gene, various mechanisms have been proposed. In S. meliloti, 441 predicted asRNAs overlapped the 5′-UTR of the associated mRNA (Additional file 2: Table S2). These may function as described for SymR in E. coli and RnaG in Shigella flexneri: cis-encoded asRNAs, antisense to 5′-UTR domains of their relative target genes, are able to modulate transcription, translation efficiency, and mRNA stability [54, 55]. In S. meliloti, 250 asRNAs overlap the 3′-UTR of their particular target genes (Additional file 2: Table S2) and therefore, might influence the target mRNA stability in a similar fashion as described for the RatA/TxpA toxin-antitoxin system in B. subtilis. Duplex formation by ratA and txpA transcripts leads to txpA mRNA degradation, and thus prevents toxin synthesis [56, 57]. The largest group of cis-encoded asRNAs in S. meliloti (n=2,266) comprises transcripts antisense to the protein-coding domain of their target mRNA (Additional file 2: Table S2). Several regulatory mechanisms have been postulated for this type of asRNA. An example of targeted co-degradation of an mRNA/asRNA duplex is illustrated by isiA/IsrR of Synechocystis sp. PCC6803 [58, 59]. Other regulatory mechanisms do not focus on the asRNAs themselves, but on the strength of their respective promoters, RNAP elongating rates, and RNAP competition events. Three mechanisms of transcriptional interference, promoter collision, promoter occlusion, and “sitting duck” interference (the dislodgement of RNAP slowly initiating transcription from one promoter by an elongating RNAP from another promoter), were proposed to explain the interfering effects of RNAP complexes acting in opposite directions .
sTSS (TSS of trans-encoded sRNAs)
Trans-encoded sRNAs are usually located in IGRs, and in contrast to antisense transcripts, do not overlap their target genes. In total, 605 sTSS were associated with trans-encoded sRNAs (Figure 1b; Additional file 2: Table S2). As described for SmelA075, SmelA060, and SmelA072 in S. meliloti, and GadY in E. coli, processed variants of non-coding transcripts are not unusual in bacteria [17, 61]. Thus, we assigned closely neighboring TSS to a single sRNA region. An example for newly identified SMa_sRNA_136 is shown in Figure 1e. The majority of trans-encoded sRNAs (n=362) were assigned only a single TSS, while 78 exhibited at least one alternative TSS (Figure 1c; Additional file 2: Table S2). Therefore, our RNAseq approach identified 440 sRNAs located in 302 IGRs (Figure 1c; Additional file 2: Table S2). Newly identifed sRNAs were named following the scheme SMx_sRNA_x and added to the S. meliloti GenDB database .
Comparison of our RNAseq approach to that of Schlüter et al. , confirmed 259 mTSS, 29 sTSS, 20 asTSS, and 43 seTSS (Figure 2c; Additional file 2: Table S2). For further validation, we compiled an additional set of transcripts from the previous 454 RNAseq data , but applied less stringent criteria (Methods). Comparison of the additional set of transcripts to those of this study showed concordance for 517 (Additional file 2: Table S2). For transcripts identified in both data sets, locations of the 3′ ends were retrieved from the previous 454 RNAseq data and are provided in Additional file 2: Table S2. Examples of four such transcripts are shown in Figure 2c.
Our RNAseq analysis revealed 440 sRNAs; therefore, the ratio of CDS to trans-encoded sRNAs in the S. meliloti genome is 14.3 (Figure 1c; Additional file 2: Table S2). Somewhat lower CDS/trans-encoded sRNA ratios were observed in V. cholerae, Anabaena sp. PCC7120, and Synechocystis sp. PCC6803, with proportions of 8, 4.4, and 10, respectively [5, 6, 48]. In S. meliloti, the majority of sRNA genes (n=180) are located as single sRNA loci in a single IGR. However, 85 IGRs harbor at least two or three and 37 IGRs harbor at least four sRNA genes (Figure 1c).
Although pSymA represents only 25.2% of the total genome size in bp, 40.9% of the trans-encoded sRNAs identified in this study mapped to pSymA, indicating an over-representation of sRNA genes on pSymA and an under-representation on the chromosome (40.7%) and pSymB (18.4%) (Figure 1b; Additional file 2: Table S2). Considering that many genes required for symbiosis are located on pSymA , it is tempting to speculate that trans-encoded sRNAs play an important role in post-transcriptional regulation of the symbiotic genes.
Aside from the previously identified 6S RNA (SMc_sRNA_307), the signal recognition particle (SMc_asRNA_791), and the tmRNA (SMc_sRNA_283) , assigning functions to sRNAs remains a complex challenge. This study extends our knowledge of sRNAs and 5′-UTRs and consequently will facilitate prospective functional analyses of sRNA/5′-UTR interactions.
Comparison to published TSS data
We compared 124 S. meliloti 1021 TSS, published over the past several decades, to our RNAseq TSS (Additional file 2: Table S5). This set of previously published TSS is biased toward rpoH-dependent genes because 69 of the 124 TSS were reported in a single study . Of the 124 published TSS, 60% matched an RNAseq TSS exactly, 11% differed by only 1–4 nt, and 7% differed by ≥5 nt. The remaining 27 previously reported TSS were not identified in our RNAseq data. Some of these may be explained by the different growth conditions tested in each study. For example, fixA and nifH are expressed primarily in symbiosis, a condition that was not included in our study for technical reasons. Additionally, Barnett et al.  used different growth media than we did, which may explain why we failed to identify 11 rpoH-dependent TSS. Two genes, nodD3 and syrA, previously reported to have low expression and extremely long 5′-UTR [63, 64], were also absent in our RNAseq data. We identified a TSS for ndvA in our RNAseq data that was misclassified by our automated system as belonging to the 5′-UTR of an asRNA (Additional file 2: Table S5). Other reported TSS, such as those corresponding to hypM, rpoN, and trkH, had matching reads in our RNAseq data, yet failed to meet the coverage cutoff. These examples illustrate the delicate balance between sensitivity and specificity in global studies; in our study, a cutoff of ≥30 reads was chosen to provide the best balance between identification of true positives and background noise.
As previously discussed, a major strength of our study is the comprehensiveness of our data. Depending on the location of the specific primer(s) chosen, alternate TSS may be missed by primer extension or 5′ RACE mapping. Hence, in comparing our TSS data to published reports, we identified 45 genes with multiple TSS, where just one TSS had been reported before (Additional file 2: Table S5). In sum, the TSS identified in this study are in good agreement with previous reports.
The ~17,000 TSS identified with RNAseq are an excellent resource with which to increase our knowledge about promoter properties in S. meliloti. As described above, previous promoter mapping has focused on regions upstream of a limited number of protein-coding genes. In addition, bioinformatics-based predictions have disregarded promoter motifs not associated with, or in antisense orientation to, protein-coding genes [27, 62, 65]. However in this study, TSS corresponding to ~3,400 asRNAs or sRNAs allowed us to directly identify 724 promoter sequences upstream of these genes, in addition to 1,371 promoters identified upstream of protein-coding (mTSS and lmTSS) genes (Figures 1c and 3a).
The σ subunit of RNAP confers promoter specificity through interaction with conserved sequences upstream of TSS . The S. meliloti genome encodes 15 σ factors: 14 of these belong to the σ70 family, and thus are predicted to recognize -35/-10-type promoters, while one (RpoN) belongs to the σ54 family and recognizes -24/-12-type promoters. Putative promoter consensuses have been identified corresponding to seven of the 15 S. meliloti σ factors (σE1, σE2, σE9, σH1, σH2, σ54, and σ70), and for promoters recognized by both σH1 and σH2 (σH1/2).
Our promoter prediction procedure is illustrated in Additional file 1: Figure S3 and described in detail in Methods. Briefly, previously identified promoter sequences for σ70, σH1, σH2, σH1/2, σ54, and σE2 were used to calculate position-specific scoring matrices (PSSM) [27, 62, 65], which were then used in a genome-wide search for promoter motifs. The resulting motifs were correlated with the locations of all mapped TSS and deemed to be putative promoters if located in the appropriate position relative to the TSS (-24/-12 for σ54, -35/-10 for all others; Methods). For prediction of σE1 and σE9 promoters, we used a different approach. These two σ factors belong to the ECF class of σ factors, which are often autoregulatory on their own operons . We had previously shown that expression of rpoE1 and rpoE4 is dramatically increased in S. meliloti 1021, compared to S. meliloti 2011  due to a loss-of-function mutation in ecfR1, encoding the putative RpoE1 anti-σ factor (Krol and Becker, unpublished results) . This suggested that RpoE1 autoregulates expression of its own operon and that of rpoE4. Examination of regions upstream of the TSS for these two operons revealed identical motifs (GAAT-N18-GTCT). This motif was used in global string searches to identify additional putative σE1 motifs upstream of TSS (Methods). For RpoE9, we also performed string searching, but with the promoter motif recently predicted in , TGTCACA-N16-CGTC, which is located 9 nt upstream of the TSS we identified for the SMb20029-rpoE9 operon.
Overall, we predicted 2,847 promoter sequences upstream of TSS (Figure 3a; Additional file 3: Tables S6-S13). σ70-dependent promoters make up the largest group of motifs (1,087, with 789 of these specific for σ70 only; Figure 3a; Additional file 3: Table S6). Similarity between the S. meliloti σ70 and σH promoter consensuses was previously noted , thus as expected, we found significant overlap (n=298) between the σ70 and σH promoter sets (Figures 3a and 3b). E. coli σ70 and σ32 promoter consensuses also share similar features , demonstrating that such overlap is not limited to S. meliloti, and that any in silico promoter prediction must be validated experimentally. In 2006, the first genome-wide prediction of S. meliloti σ70 promoter motifs provided a set of 117 experimentally validated (n=25) or computationally predicted (n=92) promoter motifs . We confirmed that 55 of their 117 promoter sequences matched our TSS and σ70 promoter predictions. Ten promoter sequences identified in their study were not associated with mTSS in our study, but instead to TSS of other categories.
RpoH-dependent promoter motifs (σH1, σH2, σH1/2)  were assigned to 1,556 unique TSS, of which 298 were also identified in searches with the σ70 promoter motif (Figure 3a; Additional file 3: Tables S7-S9). We identified extensive overlap among σH1, σH2, and σH1/2 promoter predictions (Figure 3b; Additional file 3: Tables S7-S9). Barnett et al.  characterized the RpoH1 and RpoH2 regulons during heat shock and stationary phase growth: in addition to the experimental validation of 69 TSS downstream of putative RpoH-dependent promoters (51 of which were confirmed in this study), they predicted 75 putative promoters upstream of protein-coding genes . Our data set validated ~59% (n=44) of these predicted promoters and added 647 previously unknown RpoH promoter motifs upstream of mRNA start sites (mTSS or lmTSS). Thirty-three σH promoter motifs are located upstream of rpoH-dependent genes, but were not previously identified by Barnett et al. . Due to the similarity of RpoH and RpoD promoter motifs, the remaining set of 614 predicted RpoH promoters likely includes many false positives. RpoH-dependent regulation of the small non-coding RNAs SmelC781 and SmelC456 was proposed , and indeed, our analysis identified σH1, σH2, and σH1/2 binding motifs upstream of SmelC781 and SmelC456 (Additional file 2: Table S2).
RpoN (σ54)-type σ factors are unique in that they require an activator to initiate transcription . These activators, known as enhancer-binding proteins (EBP), interact with σ54 and bind DNA upstream of the RpoN-target promoters . The S. meliloti genome is predicted to encode seven EBP (NifA, DctD, NtrC, NtrX, TacA, SMb20102, and SMb21200), but target genes have been identified for only the first three of these (reviewed in ). We identified RpoN-dependent promoter motifs (σ54) upstream of 112 TSS (Additional file 3: Table S10). Due to the lack of symbiotic samples in our RNA pools, we did not identify TSS upstream of the RpoN-dependent genes nifA, nifB, nifH, glnII and SMa0872. Only four of our predicted promoters (dctA, glnB, glnK, SMb20436) were previously characterized as RpoN-dependent or predicted by in silico methods ; therefore, our data provide a useful resource for the identification of additional RpoN-regulated genes and characterization of EBP.
For σE2, 346 promoters were predicted (Additional file 3: Table S11), of which 47 were previously found by Sauviac et al. . An additional 58 of these promoters were experimentally validated for rpoE2-dependence by microarray (Figure 3c; see below). Furthermore, we identified 41 putative σE1 promoter motifs (Additional file 3: Table S12). In contrast, only two additional promoter motifs were predicted for σE9 (Additional file 3: Table S13). This was not unexpected, as the RpoE9-type σ factors of Rhodobacter sphaeroides and Bacillus licheniformis were proposed to activate only their own operons .
Using our large set of newly predicted promoter motifs, we recompiled each of the consensus sequences for σ70, σ54, σE2, σH1, σH2, and σH1/2. As expected, the resulting motifs (Additional file 1: Figure S4) were similar to the previously reported consensus sequences [27, 62, 65]. As described before, the σ70 −10 region is poorly conserved in S. meliloti[62, 65] (Additional file 1: Figure S4).
Global identification of promoter motifs in S. meliloti was hitherto limited due to limited knowledge about TSS of individual genes. Combining the TSS identified in this study with the previously identified sRNAs  provided a rich resource for identification of promoters and their assignment to σ factors. In summary, we were able to identify promoter motifs preceding ~17.5% (1,100 of 6,296; Additional file 3: Tables S6-S13) of known protein-coding genes  and 633 non-coding RNA genes (131 sRNA and 502 asRNA). We also identified 632 promoter motifs preceding 502 DNA regions corresponding to sense transcripts (distinct seTSS with one or more promoters). This finding supports the hypothesis that at least a small percentage of sense transcripts may represent intact transcripts, such as regulatory sRNAs or mRNAs that are transcribed from promoters internal to the predicted ORF .
Transcription factor binding sites
While the σ subunit of RNAP is the primary means of conferring specific transcript initiation, it has long been known that various transcription factors interact with bacterial promoters to activate or repress transcription . Activator-dependent promoters are common among those recognized by σ70 and often possess defective promoter elements . Promoter searches using PSSM may fail to detect promoters possessing atypical core elements; therefore, understanding the mechanisms by which activators and repressors act at promoters is essential for a complete view of any transcriptional landscape. Unfortunately, such mechanisms, including specific transcription factor binding sites, are quite diverse and difficult to detect de novo on a global scale. However, TSS data can be used to provide information on promoter structure where binding sites are predicted or known, and to guide discovery of transcription factor binding sites where some functional information exists.
Additional file 4: Table S14 correlates previously reported transcription factor binding sites  with our TSS data. The group of predicted PhoB binding sites illustrates how TSS information can provide supporting empirical evidence for in silico binding site predictions. Under phosphate (Pi) limitation, the PhoR histidine kinase phosphorylates its cognate response regulator, PhoB, which interacts with conserved motifs (PhoB boxes) upstream of genes involved in the Pi starvation response. While a large regulon of genes involved in S. meliloti response to Pi limitation has been identified, and several dozen PhoB boxes have been predicted [71, 72], TSS have been determined for only three PhoB-dependent genes (phoC, phoX, and pstS in Additional file 2: Table S5). In E. coli, the PhoB box overlaps and replaces the −35 σ70 recognition elements of PhoB-dependent promoters . Since the three S. meliloti PhoB-dependent genes with mapped TSS appeared to have poor −35 σ70 recognition elements overlapping with PhoB motifs, we matched the locations of previously predicted PhoB boxes to our TSS. Of the 33 genes with predicted PhoB boxes and TSS in this study, 16 overlapped the −35 motif (i.e. were located 22 to 25 nt upstream of the TSS); and therefore, are strong candidates for PhoB binding sites (Additional file 4: Table S14). Additional PhoB boxes are located farther upstream of TSS; these may be targets for other types of regulation, for example, PhoB-mediated repression, as was proposed for SMc02862 .
An example of how TSS data may guide binding site discovery is illustrated by the example of CtrA, a global cell cycle regulator. CtrA is autoregulatory upon its own promoter, which contains five verified CtrA binding sites (Figure 1d) . In contrast to C. crescentus, where the CtrA regulatory circuit is well characterized , little is known about CtrA targets in S. meliloti. We used PSSM to locate additional putative CtrA binding sites upstream of S. meliloti protein-coding genes and compared these to our TSS data (Methods). We identified 175 putative binding motifs, representing 158 genes: ~70% of the motifs are located upstream of TSS or overlap TSS (Additional file 4: Table S15). We confirmed CtrA motifs upstream of TSS corresponding to S. meliloti cell cycle-related genes previously predicted to possess such motifs (minC, chpT, rcdA, pleC) [76, 77], and identified CtrA motifs upstream of rpoD and ftsE, previously shown to bind CtrA in Brucella abortus. Other S. meliloti genes with CtrA motifs that are plausibly cell cycle regulated or were shown to be direct CtrA targets in C. crescentus include podJ, mraZ, metK, clpP2, ftsK, flaA, flaC, flaD, mcpE, mcpY, and SMc00651 (Additional file 4: Table S15). Our data also suggest potential regulatory mechanisms; for example, S. meliloti gcrA, an ortholog of C. crescentus gcrA encoding a master cell cycle regulator that activates ctrA transcription , is transcribed divergently from argD and possesses a strong CtrA motif overlapping the gcrA TSS, but on the opposite strand. A weaker CtrA motif that did not make our cutoff (TAA-N7-TTACT; P-value = 3.4×10-4) is located on the same strand as the gcrA TSS and almost completely overlaps the strong motif. The regulatory significance of this arrangement is unknown, but we speculate that CtrA may mediate a complex mechanism of both activation and repression at the gcrA promoter.
de novopromoter motif discovery
Of the 4,925 protein-coding genes for which we did not identify a promoter, 3,468 lacked TSS with ≥30 reads. The remaining 1,457 genes had one or more TSS (mTSS or lmTSS), but lacked an upstream promoter prediction. These may represent genes transcribed by σ70, σ54, σE1, σE2, σE9, σH1, or σH2, but whose promoters contain atypical core motifs, or genes whose promoters are recognized by one more of the other eight S. meliloti σ factors (σE3, σE4, σE5, σE6, σE7, σE8, σE10, and σfecI). In order to determine whether any of these genes lacking a promoter prediction share similar, as yet to be identified promoter motifs, we extracted sequences 40 nt upstream of high coverage TSS (≥300 reads) and used them as input for MEME ; Methods). Using this set of 482 upstream sequences, we identified three motifs with E-values of < 1 (Additional file 1: Figure S5). Motif 1 was identified upstream of 159 genes and consists of a conserved upstream TTG and a conserved downstream A residue (Additional file 1: Figure S5). In addition to genes lacking an annotated function (~40%), the list includes genes involved in housekeeping, transport, metabolic, and regulatory functions (Additional file 4: Table S16). Therefore, we speculate that Motif 1 corresponds to genes transcribed by RpoD that possess a conserved TTG motif, but lack other features of the RpoD consensus sequence (Additional file 1: Figure S4). Motif 2 contains a central TTTGTTAACCAT sequence and was identified upstream of 19 genes (Additional file 1: Figure S5; Additional file 4: Table S16), 84% of which were previously shown to have high expression in rich medium, yet decreased expression in nodule bacteria and during heat shock [62, 80]. Motif 2 does not appear to match any previously identified S. meliloti promoter motifs or any motifs in the manually curated prokaryotic PSSM database, RegTransBase . Motif 3 (TTCA-N7-TTCA) was identified upstream of 12 genes (Additional file 1: Figure S5; Additional file 4: Table S16), five of which were previously identified as FeuP-dependent . FeuP encodes a response regulator required for bacterial invasion of root nodules and activation of at least 14 genes , including ndvA encoding a cyclic σ-glucan exporter, and feuN, a negative modulator of the FeuPQ pathway that is predicted to be cotranscribed with feuPQ (Additional file 4: Table S17) . We checked whether Motif 3 was present upstream of the remaining nine FeuP-dependent genes: three (including feuN) had motifs in appropriate distance upstream of TSS and three had motifs upstream of ORFs for which TSS were not identified (Additional file 4: Table S17). Therefore, we suggest that Motif 3 is a candidate FeuP binding site. In sum, our identification of three novel motifs upstream of TSS demonstrates the utility of global TSS data as a discovery tool.
The S. meliloti RpoE2 (σE2) regulon
The S. meliloti ECF σ factor, RpoE2 (σE2), responds to heat shock, osmotic stress, oxidative stress, and carbon/nitrogen starvation during stationary phase growth [27, 84], activating expression of at least 45 genes . Most α-proteobacteria possess RpoE2-like σ factors and their role was proposed to be analogous to that of RpoS in E. coli. The activity of σE2 is controlled by a partner switching mechanism, which includes negative regulation via two paralogous anti-σ factors, RsiA1 (SMc01505) and RsiA2 (SMc04884), and positive regulation via two anti-anti-σ factors, RsiB1 (SMc01504) and RsiB2 (SMc00794) [27, 86]. RsiB1 and RsiB2 each contain a C-terminal receiver domain, which is phosphorylated by an unidentified histidine kinase(s), allowing the N-terminal ECF σ-like domain to interact with RsiA1 or RsiA2, thereby relieving inhibition of σE2.
A previous study identified rpoE2-dependent genes in S. meliloti 1021 by comparing transcription profiles of an rpoE2 mutant and wild type during heat shock . To identify additional RpoE2 target genes, independent of any specific stress condition, and to verify RpoE2-dependent regulation of genes associated with putative σE2 TSS identified in this study, we used custom Affymetrix GeneChips to obtain transcription profiles of S. meliloti strains either overexpressing rpoE2 from an inducible promoter or carrying the empty vector (Methods). As mentioned above, S. meliloti 1021 has a defective ecfR1 gene, resulting in high constitutive RpoE1 (σE1) activity. Sigma factors compete with each other for RNAP ; therefore, to maximize the amount of RNAP-σE2, and presumably enhance identification of σE2 targets, we performed our experiments in a strain containing a functional ecfR1 gene (CL150; Methods).
Our analyses revealed that 202 protein-coding genes displayed more than twofold increased transcript abundance in the strain overexpressing rpoE2, whereas three mRNAs showed lower abundance (Additional file 5: Table S18). The majority of the protein-coding genes (n=150) lack a predicted function (Additional file 5: Table S18). About 95% of rpoE2-dependent transcripts previously identified by microarray , showed increased expression in the rpoE2 overexpressing strain. In addition, we identified 161 new rpoE2-dependent protein-coding genes (fold change ≥2), 41 of which confirm previous in silico predictions . Overall, ~72% of rpoE2-dependent protein-coding genes had one or more mapped TSS in our RNAseq data (Additional file 5: Tables S18 and S20).
As expected, expression of regulatory genes rpoH2 (SMc03873), rpoE5 (SMb21484), rsiA1 (SMc01505), and rsiB1 (SMc01504) was rpoE2-dependent; moreover, each of these genes has an mTSS downstream from an RpoE2-dependent promoter (Figure 4a; Additional file 5: Table S19). In addition, we identified TSS with σE2 motifs upstream of two operons encoding rpoE2-dependent response regulator-histidine kinase pairs: SMa0113/114 and exsFG (SMb20933/934; Additional file 5: Table S19). These observations demonstrate the complexity of the RpoE2 regulatory circuit and suggest that rpoE2 overexpression may result in multiple, secondary regulatory effects. Thus, 76 rpoE2-dependent protein-coding genes possess a TSS preceded by a σE2-binding motif: these are likely directly controlled by σE2, while transcription of the remaining genes likely depends on other σ factors (Figures 4a and 4c, Additional file 5: Table S19). For example, 22 rpoE2-dependent operons were previously shown to be rpoH-dependent . Fifteen (68%) of these had an RNAseq TSS preceded by a promoter prediction for RpoE2 (n=5), RpoH (n=9), or both (n=1) (Additional file 5: Tables S18 and S19).
In addition to detecting mRNAs corresponding to protein-coding genes, our custom Affymetrix chip detects transcriptional activity for IGRs ≥ 150 nt. The strain overexpressing rpoE2 showed increased hybridization, compared to the control strain, to 63 probe sets, corresponding to 56 IGRs, and decreased hybridization to two probe sets (Figure 3c; Additional file 5: Tables S18 and S20). Our RNAseq approach detected transcripts corresponding to 43 of these IGRs. About 60% of IGRs showing rpoE2-dependent hybridization are adjacent to rpoE2-dependent protein-coding genes, and therefore likely represent 5′- or 3′-UTR of those genes (Figure 3c; Additional file 5:Tables S18 and S20). IGRs corresponding to 5′-UTRs of six genes SMa0022, SMa2357, SMb20413, SMb20705, SMc00794, and SMc00922 showed increased expression in the rpoE2 overexpressing strain that did not correlate with that of their corresponding coding regions (Figure 3c; Additional file 5: Table S18); however, we confirmed rpoE2 dependence for three of these by 5′ RACE mapping (SMa2357, SMb20705, SMc00922; see below). Five protein-coding genes, newly identified in this study, correlated with rpoE2-dependent IGRs identified by Affymetrix analysis (Figure 4c; Additional file 5: Table S20).
σE2 promoter motifs were predicted upstream of 23 sRNAs (Figure 3a, Additional file 5: Table S20). Our microarray data provides evidence for rpoE2-dependent transcription in eight IGRs where sRNA genes are located: SmelA018, SmelA060, SMa_sRNA_126, SMb_sRNA_381, SMb_sRNA_432 (SmelB126), SMb_sRNA_433 (Smel-B127ov), SMc_sRNA_259, and SMc_sRNA_298 (Figures 3c and 4c; Additional file 5: Table S20). This suggests that sRNA mediated post-transcriptional control is part of the RpoE2 regulatory circuit.
σE2 promoter motifs were identified upstream of 40 asRNAs (Figure 3a; Additional file 3: Table S11). At the post-transcriptional level, cis-encoded asRNAs and trans-encoded sRNAs may play a role in complex regulatory circuits by allowing for interference between transcripts of different σ factor regulons. For example, eight rpoE2-dependent asRNAs are located in antisense to genes are predicted to be controlled by σ70, σH or both (Figure 5a). Figure 5b shows an example for the σE2-dependent SMc_asRNA_904, which may interact with the σ70-dependent SMc02217 mRNA. In addition, 70 asRNAs were found in antisense to rpoE2-dependent genes. We predicted binding motifs for σ70, σH, or both, upstream of 17 of these asRNAs. An example is the σ70-dependent SMc_asRNA_1559, which may interact with the rpoE2-dependent SMc04232 mRNA (Figures 5a and 5b). These observations strongly support the hypothesis that asRNAs belonging to a distinct σ factor regulon can interact with targets of different σ factor regulons.
5′ RACE mapping of rpoE2-dependent transcripts
To confirm RNAseq and Affymetrix data, we chose 26 genes for 5′ RACE (random amplification of cDNA ends) mapping (Methods). For these experiments, we used the same RNA samples as were used for the Affymetrix analyses. Because IGR probe sets on our custom Affymetrix GeneChip are a low-resolution means of delineating transcript structure, we examined TSS and rpoE2 dependence for putative sRNAs, newly identified ORFs, and 5′-UTR detected by these IGR probe sets. Also, since RpoE2 was shown to activate expression of rpoH2, we tested seven rpoE2-dependent genes whose expression was previously shown to be rpoH-dependent . As controls, we included two regulatory genes whose expression was not rpoE2-dependent, rpoH1 and rsiA2. Results of 5′ RACE mapping are provided in Additional file 5: Table S21, and gel photos showing results for four representative transcripts are shown in Additional file 1: Figure S6. Of the 26 RACE mapped genes, 24 had TSS in the RNAseq data, and all but three of these TSS matched our RACE determined start sites exactly. rpoE2 dependence was confirmed qualitatively by 5′ RACE for all genes tested except for SMb20413, and as expected, rpoH1 and rsiA2. Most mapped promoters had upstream matches to the RpoE2 promoter consensus sequence, thus the corresponding genes are likely direct targets of RpoE2. Two genes previously identified as rpoH-dependent (SMc01507 and SMc03968; ), had RpoH-like promoters.
To our knowledge, this study reports the first genome-wide RNAseq identification of TSS in an α-proteobacterium. Our approach defined a set of 17,001 TSS that provides mRNA start sites for ~45% of S. meliloti protein-coding genes and identifies new ORFs and ncRNAs, including asRNAs complementary to about one third of protein-coding genes. Over 2,000 TSS are preceded by at least one predicted promoter sequence, representing potential target promoters for nearly half of the known S. meliloti σ factors. As promoter consensus sequences become available for the remaining σ factors, our data set can be used to identify target genes of these σ factors. Also, we demonstrated how TSS identification on a global scale aids in discovery of novel promoter motifs and transcription factor binding sites. Combined with our Affymetrix GeneChip analyses, the RNAseq data expand the known regulon of the σ factor, RpoE2, and identify candidate ncRNAs that may be involved in the S. meliloti general stress response. In sum, our work provides a rich resource for continued study of S. meliloti gene expression and regulatory circuits, as well as a foundation for comparative studies of transcription in other α-proteobacterial species.
Strains and growth conditions for RNAseq experiments
The sequenced reference strain, S. meliloti strain 1021 [20, 87], and S. meliloti strain 1021expR+ were used for the RNAseq experiments. S. meliloti strain 1021expR+ was constructed by replacing expR, disrupted in 1021 by an insertion element , with a functional expR gene. To repair expR, the corresponding genomic sequence of strain Rm8530  was amplified using primers 5′-ACACAAGCTTCTTCTGAACGGCGTATTCACA and 5′-TGATGAATTCCATTCCGTCGGCGAGATAGT and cloned into the HindIII and EcoRI restriction sites of pK18mobsac . The construct was introduced into the genome of Rm1021 by conjugation. Transconjugants were subjected to sucrose selection on LB (Luria-Bertani) agar plates  with 10% sucrose, which allowed for selection of the 1021expR+ strain.
For large-scale identification of TSS in the genome of S. meliloti 1021, RNA samples representing 16 different growth and stress conditions, each in three biological replicates, were purified and pooled. Unless stated otherwise, 50 ml cultures of S. meliloti strains 1021 and 1021expR+ were inoculated to a starting OD600=0.02 in 250 ml flasks and incubated at 30°C with shaking (180 rpm) in TY , VMM  or MOPS-MM medium , supplemented with 8 μg/ml nalidixic acid.
Exponential and stationary phase RNA samples were purified from S. meliloti 1021 cultures grown in TY (OD600=0.8 or 3), VMM (OD600=0.6 or 1.3), and MOPS-MM (OD600=0.5). Exponential phase cultures of S. meliloti 1021expR+ were grown in MOPS-MM (OD600=0.5). For exposure to various environmental stresses, the following modifications were made. All stress treatments were applied to strain 1021 only, unless noted otherwise:
Temperature shifts for heat (40°C) and cold shock (20°C) were applied for 30 min to cultures grown in TY.
Exposure to microoxia was performed by flushing TY-grown cultures with pure nitrogen (N2) for 1-minute, followed by incubation of cultures under a N2 atmosphere for 45 minutes.
Salt stress was carried out by adding sodium chloride (NaCl) to exponential phase, VMM-grown cultures at final concentration of 0.4 M for 20 minutes. Oxidative stress exposure was performed similarly, except instead of NaCl, H2O2 was added to a final concentration of 10 mM.
Exposure to acid and alkaline stress was as follows: cultures were grown to an OD600 of 0.6, centrifuged, and the resulting cell pellets resuspended in VMM modified by addition of either HCl to pH 5.8 or NaOH to pH 8.5.
Cultures were starved for nitrogen or carbon by growing them to an OD600 of 0.6 in replete MOPS-MM, followed by centrifugation and resuspension of the cell pellets in MOPS-MM lacking either a nitrogen or carbon source . S. meliloti 1021 and 1021expR+ cultures were subjected to phosphate limitation in MOPS-MM with 0.1 mM phosphate as described previously .
For induction with the flavonoid luteolin, cultures were grown in TY to an OD600 of 0.8, luteolin was added to a final concentration of 10 μM, and cells were harvested after 4 hours incubation.
RNA preparation for RNAseq
Total RNA was isolated using miRNeasy Mini kits and a QIAcube automated nucleic acid preparation platform, according to manufacturer’s instructions (Qiagen). RNA samples were further purified by phenol/chloroform/isoamyl alcohol extraction and ethanol precipitation. The integrity of all RNA samples was confirmed using a RNA 6000 Nano Kit with a Bioanalyzer 2100 (Agilent Technologies).
cDNA library preparation and RNAseq
The pooled RNA sample was sequentially treated with two enzymes: (i) terminator 5′-phosphate-dependent exonuclease (TPE; Epicentre), which specifically degrades RNA species with 5′ monophosphates (processed transcripts), and (ii) tobacco acid pyrophosphatase (TAP; Epicentre), which prepares the TPE-resistant transcripts from (i) for adapter ligation by removing pyrophosphates from their 5′ ends. Subsequently, an adapter comprised of sequences complementary to the sequencing and amplification primers was ligated to the 5′ phosphate of the pretreated mRNA. First-strand cDNA synthesis was then performed with an N6 randomized adapter primer and M-MLV-RNase H reverse transcriptase (New England Biolabs). The resulting cDNA was PCR-amplified in 24 cycles. The primers used for PCR amplification were designed for amplicon sequencing according to Illumina/Solexa guidelines. The following adapter sequences flanked the cDNA inserts: 5′ end, 5′- A ATGATACGGCGACCACCGACAGGTTCAGAGTTCTA CAGTCCGACGATCTCCA-3′ and 3′ end, 5′- CAAG CAGAAGACGGCATACGATCAGGCAGAGGACGAGAA-3′ (Illumina adapter sequences are underlined). Prior to sequencing, double stranded cDNA was enriched for fragments of 300 to 500 nt (the optimal range for our sequencing method) by size fractionation. RNAseq was performed on the Illumina HiSeq 2000 sequencing system by GATC Biotech (Konstanz, Germany).
We note that while our procedure resulted in an enrichment of primary 5′ ends, such enrichment is never complete. Hence, a detectable proportion of a given abundant transcript with a processed 5′ end can survive the enrichment procedure. In addition, the specific tertiary structure of some processed RNAs may result in their 5′ ends being stably protected against TPE degradation. Therefore, for some genes, both primary and processed transcripts may be represented in our data set.
Identification of transcription start sites (TSS)
Sequences of the S. meliloti 1021 genome, accession numbers NC_003037 (pSymA), NC_003047 (chromosome), NC_003078 (pSymB), and gene annotations, including the set of sRNAs previously identified by 454 sequencing , were downloaded from NCBI and the RhizoGate Portal , respectively.
Sequencing reads from the cDNA library were processed and mapped to the S. meliloti 1021 genome using segemehl . From an initial set of 37,792,608 reads, 35,043,949 reads ≥ 18 nt were mapped to the reference sequence. To enrich for the number of reads originating from a TSS (the 5′ end of a transcript), only reads that mapped to a unique position in the genome, and without mismatches in the first three bases of the 5′ end, were retained for downstream analysis. This resulted in a final set of 11,230,166 reads. The overall workflow is outlined in Additional file 1: Figure S1.
The next step in the workflow was to identify TSS. We assembled reads into TSS contigs, assemblies of at least 30 mapped reads sharing a common 5′ end. Thus, the 5′ end of a TSS contig constitutes a TSS, while the 3′ end of the longest read determines the end position of the TSS contig. If the distance of two TSS positions differed by less than 3 nt, they were treated as a single TSS and merged. Altogether, we identified 17,001 TSS contigs: 15,056 that originated from a single TSS contig, and 1,945 that were assembled from two or more TSS contigs. TSS were named using the scheme: SMx_TSS_nnnn where x = A, B or C and denotes a location on pSymA, pSymB or the chromosome, respectively.
Based on a minimal transcriptional unit (MTU) model, we derived six classes of TSS: lmTSS, mTSS, pmTSS, seTSS, asTSS, and sTSS (see below). These classes reflect the relative position and orientation of a TSS contig to its genomic context. The TSS classes are organized hierarchically to guarantee that TSS contigs that meet definitions of multiple classes are assigned to a single class.
The MTU of a gene is divided in three consecutive regions: 5′-untranslated region (UTR), coding sequence (CDS), and 3′-UTR. Nucleotide numbering starts with 1 at the first nucleotide of the 5′-UTR. The size of the coding segment is delimited by the position of its start and stop codon. In contrast, we used fixed length thresholds for the UTRs, which represent the minimal required sizes of ribosome binding sites (RBS; 14 nt) and terminator hairpins (20 nt) within the 5′-UTR and the 3′-UTR, respectively. The promoter region upstream of the MTU comprises nucleotides from position -40 to -1.
TSS class definitions
These TSS are probably associated with mRNAs. To associate identified TSS with protein-coding genes, the defined minimal length of 14 nt of the 5′-UTR, the defined minimal length of 40 additional nt for the promoter region, and the length range of the sequence contigs assembled from our data were taken into account. Contigs ranged from 87 to 108 nt. If a contig was in the same orientation and overlapped the minimal region of 14 plus 40 nt upstream of the start codon, we assumed that it is more likely associated to an mRNA than to a trans-encoded sRNA and therefore classified its prominent 5′ end as an mTSS.
Also, to identify additional mTSS, we included cis-encoded mRNA leader sequences from the 454 RNAseq data  in our analyses (see below). Thus, a TSS contig, which is located upstream of a promoter region and without overlapping it, is categorized as mTSS, if there exists a cis-encoded mRNA leader sequence for this MTU that starts at the same position or upstream of the mTSS.
These TSS are associated with leaderless transcripts and match the first nucleotide of the corresponding AUG start codon.
These represent a class of putative mTSS where it is uncertain if the TSS belongs to an mRNA or to the transcript of an sRNA. This classification is used because TSS located over 300 nt away from the corresponding start codon are rarely observed. TSS contigs of pmTSS do not overlap with any MTU in sense and antisense and are located at most 300 nt upstream in same orientation of a start codon.
Sense TSS must meet two criteria: the TSS is located within an MTU, and has the same orientation as the associated MTU. This is true for all TSS within an MTU except for those that meet the definition of the lmTSS class.
These TSS represent cis-encoded antisense RNAs. In contrast to seTSS, the asTSS contigs overlap MTUs in antisense orientation.
These TSS represent trans-encoded sRNAs located in IGRs. Therefore sTSS contigs do not overlap any MTU. In the case where an MTU is located downstream, in the same orientation, a TSS is classified as an sTSS only if the distance between start codon and TSS exceeds the pmTSS threshold of 300 nt.
Definition of trans-encoded sRNAs and cis-encoded antisense RNAs
After categorizing the TSS, we merged overlapping TSS contigs of sTSS and asTSS. The resulting trans-encoded sRNA and cis-encoded antisense RNA transcripts are named according to the following conventions, SMx_sRNA_n and SMx_asRNA_n, respectively.
Identification of new sRNAs from 454 RNAseq data
Schlüter et al.  used a 454 RNAseq approach to identify non-coding RNAs shorter than 350 nt. In that study, 454 contigs were categorized as follows: trans-encoded sRNA, cis-encoded mRNA leader, sense sRNA, and cis-encoded antisense RNA. For this study, we reanalyzed the 454 RNAseq data using less stringent parameters to identify additional sRNAs. We defined a 454 contig as a region with continuous coverage of at least 5 reads and a length between 50 and 350 nt. From this initial set, we chose only those 454 contigs whose 5′ end matched a TSS from this study. Schlüter et al.  adopted a naming convention of SmelXnnn for their sRNAs; in order to distinguish our newly identified sRNAs we inserted an R (SmelXRnnn), indicating that relaxed parameters were applied.
Comparative gene prediction
If the TSS of an organism are known, one may guide the gene annotation process by using the genomic coordinates of the TSS as constraints for gene prediction. Here, we combined our TSS data with RBS (ribosome-binding site) and open reading frame (ORF) predictions, and carried out protein similarity searches to improve the S. meliloti genome annotation by finding new genes and correcting positions of start- and stop-codons. Our procedure is presented in Additional file 1: Figure S2.
For each TSS transcript, T, we performed the following steps: First, the set of putative ORFs that overlap with T were identified. Then, we distinguished between two kinds of ORFs, depending on the translation initiation mechanism: leaderless ORFs and Shine-Dalgarno (SD) initiation ORFs (sdORFs). While a leaderless ORF possesses an AUG start codon and its 5′ end coincides with the TSS, sdORFs are preceded by a leader sequence, with the TSS as the 5′ end. Since the leader sequences contain an RBS, we set the minimum length threshold to 14 nt. In the next step, all ORF sequences were translated and matched against the NCBI non-redundant (nr) protein database using BLASTP. BLASTP hits with an E-value < 10-5 were selected if the BLASTP alignment covered the query sequence completely and if the matching protein and the query were of similar length. For sdORFs we used free_align to predict RBS on the leader sequences. free_align identifies an RBS as the energetically most favorable hybridization site of a target leader sequence with the 3′ tail of a 16S RNA by applying free energy calculations. Following Starmer et al. , we set the energy cutoff for a RBS to −3.4535 kcal/mol. Subsequently, we classified sdORFs with RBSs and leaderless ORFs as either new ORFs or reannotated ORFs. New ORFs did not overlap more than the start or stop codon of existing annotated ORFs. If an ORF O shared either the 5′ or the 3′ end, denoted by a start or stop codon, respectively, with a gene G, O was classified as a reannotated ORF. ORFs that did not fall into these two categories were discarded, as the purpose of the ORF prediction procedure was not to replace current gene annotations with another gene annotation having a different gene product. New ORFs were named following the scheme, SMx_ORF_n. All new ORFs and reannotation ORFs were included in the GenDB S. meliloti 1021 database .
Identification of promoter motifs
Promoter consensus determination and in silicogenome-wide predictions
Parameters such as spacer threshold and promoter element size used to search for putative promoter sequences specific for RpoD, RpoE2, RpoE1, RpoE9, RpoH1, RpoH2, RpoH1/2, and RpoN are listed in Additional file 5: Table S22. In contrast to previous studies, all regions upstream of TSS were included in our analyses, regardless of its position in an IGR or a CDS. To discover promoter sequences, we followed two different strategies, depending on available input data: string-based or profile searching (see below).
String-based promoter search for RpoE1 and RpoE9 promoters
We used the consensus motifs, GAAT-N18-GTCT (RpoE1; unpublished observations; ) and TGTCACA-N16-CGTC (RpoE9; ), to perform pattern matching on the S. meliloti 1021 genome. We scanned for putative promoters that had no more than a single mismatch with respect to the consensus, a spacer length in the range specified in Additional file 5: Table S22, and were located upstream of a TSS with minimum and maximum distance of 5 nt and 12 nt from the end of the promoter, respectively.
Profile search of promoters
Previously identified promoter sequences were used as input for the prediction of RpoD- (n=25), RpoH1- (n=20), RpoH2- (n=11), RpoH1/H2- (n=14), and RpoN- (n=8) specific promoters [62, 65, 98]. For the RpoN promoter search model, we excluded two that were previously reported  because one was shown to be RpoD-like and the other was not found in S. meliloti strain 1021. For RpoE2 promoters, only one RpoE2-dependent TSS, that of the rsiA1-rpoE2 operon, had been mapped prior to this study ; therefore, we used a set of 35 putative promoters predicted previously by aligning upstream regions of a set of rpoE2-dependent genes . For purposes of our study, input promoters were designated as either “virtual”, if they had been previously reported in the literature, but no TSS corresponding to the promoter was present in our RNAseq data, or as “model” if an RNAseq TSS was located an appropriate distance downstream (Additional file 3: Tables S6-S11 and Additional file 5: Table S23).
In view of the sparse promoter data, we implemented an iterative two-phase procedure to both identify the global promoter architecture and to refine the promoter consensus. The main analytical steps of our promoter prediction workflow are outlined in Additional file 1: Figure S3.
Before beginning Phase 1, we extended the set of input promoter sequences by searching for promoter regions identical to the −35 and −10 elements of each input promoter, and within an appropriate distance of a TSS (denoted “extended model ” in Additional file 3: Tables S6-S11).
In Phase 1, promoter candidates were identified by means of position-specific scoring matrices (PSSMs). A PSSM is the probabilistic representation of a promoter motif; it summarizes a conserved pattern by modeling nucleotide variability at each position of the motif. We conducted a profile search for seed promoter sequences, using the initial PSSMs obtained with the input promoter sequences. First, −35 and −10 elements were extracted from the input promoter sequences, aligned, and separate PSSMs constructed from the alignments with a pseudocount=1. After constructing PSSMs, we performed a profile search on the S. meliloti genome for putative promoter elements using PoSSuMsearch , Then, based on the promoter structure we computed chains of collinear −35 and −10 elements, such that a −35 element is located upstream of a −10 element and the distance between the elements complies with the spacer length threshold (Additional file 5: Table S22). Central to the promoter prediction process was the integration of TSS and 454 contigs  with promoter candidates. Promoter candidates were retained only if they were located 5 nt to 12 nt upstream of a TSS or 454 contig. The last filter step of Phase 1 discarded all promoters that had promoter elements with P-value > 0.005 or that were associated with seTSS (sense sRNAs) because such predictions were more likely to be false positives. This ensured that only promoters that were good representatives of their respective promoter motif were combined with the input promoter sequences to form a new set of seed promoter sequences (denoted “new from initial search” in Additional file 3: Tables S6-S11).
In Phase 2, we started with the new set of promoter sequences obtained from Phase 1. All steps of Phase 1 were then repeated with this new set and the same parameters, except for the last filter step. Since the aim of Phase 2 was to obtain a comprehensive set of promoters and to elucidate promoter architecture, we lowered the restrictions by allowing all classes of TSS to be associated with promoters and increased the P-value threshold to 0.02 (Additional file 1: Figure S3). The additional promoters identified in Phase 2 are denoted “second search” in Additional file 3: Tables S6-S11.
Identification of CtrA binding motifs
To identify putative CtrA binding sites upstream of S. meliloti protein-coding genes, we used a matrix-based search method, RSA-tools-matrix-scan . The PSSM used for searching included sequences of five experimentally verified CtrA binding sites upstream of ctrA (consensus=TAA-N7-TTAAC; ). Although one of these binding sites has 6 nt spacing, we searched only for motifs with 7 nt spacing because CtrA binding sites with spacing ≠ 7 nt showed low affinity binding in C. crescentus. We searched the direct strand of DNA upstream of all ORFs (pseudo-frequencies=0.01) and retained those hits that did not overlap ORFs and that had a positive weight score and P-value ≤ 1×10-4.
de novopromoter motif discovery
For de novo promoter motif discovery we compiled a set of 482 sequences representing 40 nt upstream of mTSS and lmTSS that were not assigned to a σ factor and had a coverage of at least 300 reads (10 fold of the coverage threshold used to identify TSS). The sequences were used as input for MEME (multiple em for motif elicitation) version 4.8.1 , with the following parameters: -dna -mod anr -minw 18 -maxw 40 -minsites 10. Motifs with an E-value of <1 were examined further.
Affymetrix GeneChip analysis and 5′RACE mapping
To identify genes whose expression was rpoE2-dependent, we used Affymetrix GeneChip analysis to compare two strains: CL150 pCAP11 and CL150 pF1084. CL150 is an S. meliloti 1021 strain in which two point mutations were corrected by gene replacement: ecfR1, encoding the RpoE1 anti-σ factor, and pstC, encoding a subunit of the high affinity phosphate transporter . To repair ecfRI, the corresponding genomic sequence of strain Rm2011  was amplified using primers 5′-CTCGAGCTGCGGAGACCGAAATGACC and 5′-CTCGAGTGCCTGGGAGAGCTATCTTG and cloned into the SmaI restriction site of pJQ200  to create pCL102P. pCL102P was introduced into the genome of strain 1021 by conjugation. Transconjugants were subjected to sucrose selection on M9 agar plates with 10% sucrose, which allowed for selection of the 1021ecfR1+ strain, designated CL101. To repair pstC, the corresponding genomic sequence of strain RmP110  was amplified using primers 5′-ATACTAGTTGTTCTTCTACGTTAAGAAGGCTC and 5′-AACTCGAGGATGAGCATGATGCCCATGACGAT and cloned into the SpeI and XhoI restriction sites of pJQ200  to create pMB772. pMB772 was introduced into the genome of strain CL101 by conjugation. Transconjugants were subjected to sucrose selection on M9 agar plates with 10% sucrose, which allowed for selection of the 1021ecfR1+, pstC+ strain, designated CL150. pCAP11 is a broad host range expression vector for exogenous expression of genes from the inducible melibiose promoter, PmelA. A plasmid overexpressing rpoE2 was constructed by amplifying the rpoE2-coding region from strain 1021 using primers 5′-GAGGATACGCGATGTCATCCGAAAACCAAG and 5′-AACACCTAGGTCACGAAACGAAGGCAC for 20 cycles, then adding the primer, 5′-GGGGCCTAGGACAGGAGGATACGCGAT, and amplifying for an additional 20 cycles. The resulting DNA was gel purified, digested with AvrII, and cloned into the AvrII site of pCAP11. Triplicate cultures of CL150 pCAP11 (vector only control) and CL150 pF1084 were inoculated to an OD600 of 0.05 in M9 glycerol medium and allowed to grow to midexponential phase (OD600=0.50-0.55), at which time melibiose was added to a final concentration of 0.4%. After 30 minutes, cells were harvested as previously described . RNA purification, cDNA synthesis, labeling, hybridization to custom Affymetrix GeneChips, and data analysis were performed as previously described . The custom dual-genome GeneChip contains probe sets corresponding to coding sequences from the original S. meliloti genome annotation reported in reference , intergenic regions (IGRs) of ≥ 150 nt, and to ~10,000 host plant (Medicago truncatula) expressed sequence tags. In designing the IGR probe sets, large IGRs were equally subdivided to be < 375 bp and tiling of oligo-(25)-mers was evenly spaced on both strands. The Affymetrix data described in this study are available in the National Center for Biotechnology Information’s Gene Expression Omnibus  through the GEO Series accession number GSE40391.
5′ RACE (5′ rapid amplification of cDNA ends) was used to determine transcription start sites for a subset of rpoE2-dependent genes, as well as for two regulatory genes whose expression was not rpoE2-dependent (rpoH1 and rsiA2). Primers used for 5′ RACE mapping are provided in Additional file 5: Table S21. Altogether, we determined transcription start sites for 26 genes, selected primarily to represent genes whose expression was detected by IGR probe sets or whose expression was previously shown to be rpoH-dependent .
Initial promoter search
Multiple em for motif elicitation
Minimal transcription unit
Open reading frame(s)
Position-specific scoring matrix
Random amplification of cDNA ends
Ribosome binding site
RNA polymerase core enzyme
small non-coding RNA
Transcription start site(s)
Waters LS, Storz G: Regulatory RNAs in bacteria. Cell. 2009, 136: 615-628.
Storz G, Vogel J, Wassarman KM: Regulation by small RNAs in bacteria: expanding frontiers. Mol Cell. 2011, 43: 880-891.
Lee DJ, Minchin SD, Busby SJW: Activating transcription in bacteria. Annu Rev Microbiol. 2012, 66: 125-152.
Sharma CM, Hoffmann S, Darfeuille F, Reignier J, Findeiss S, Sittka A, Chabas S, Reiche K, Hackermüller J, Reinhardt R, Stadler PF, Vogel J: The primary transcriptome of the major human pathogen Helicobacter pylori. Nature. 2010, 464: 250-255.
Mitschke J, Georg J, Scholz I, Sharma CM, Dienst D, Bantscheff J, Voss B, Steglich C, Wilde A, Vogel J, Hess WR: An experimentally anchored map of transcriptional start sites in the model cyanobacterium Synechocystis sp. PCC6803. Proc Natl Acad Sci USA. 2011, 108: 2124-2129.
Mitschke J, Vioque A, Haas F, Hess WR, Muro-Pastor AM: Dynamics of transcriptional start site selection during nitrogen stress-induced cell differentiation in Anabaena sp. PCC7120. Proc Natl Acad Sci USA. 2011, 108: 20130-20135.
Vijayan V, Jain IH, O’Shea EK: A high resolution map of a cyanobacterial transcriptome. Genome Biol. 2011, 12: R47-
Passalacqua KD, Varadarajan A, Ondov BD, Okou DT, Zwick ME, Bergman NH: Structure and complexity of a bacterial transcriptome. J Bacteriol. 2009, 191: 3203-3211.
Oliver HF, Orsi RH, Ponnala L, Keich U, Wang W, Sun Q, Cartinhour SW, Filiatrault MJ, Wiedmann M, Boor KJ: Deep RNA sequencing of L. monocytogenes reveals overlapping and extensive stationary phase and sigma B-dependent transcriptomes, including multiple highly transcribed noncoding RNAs. BMC Genomics. 2009, 10: 641-
Güell M, van Noort V, Yus E, Chen WH, Leigh-Bell J, Michalodimitrakis K, Yamada T, Arumugam M, Doerks T, Kühner S, Rode M, Suyama M, Schmidt S, Gavin AC, Bork P, Serrano L: Transcriptome complexity in a genome-reduced bacterium. Science. 2009, 326: 1268-1271.
Arnvig KB, Comas I, Thomson NR, Houghton J, Boshoff HI, Croucher NJ, Rose G, Perkins TT, Parkhill J, Dougan G, Young DB: Sequence-based analysis uncovers an abundance of non-coding RNA in the total transcriptome of Mycobacterium tuberculosis. PLoS Pathog. 2011, 7: e1002342-
Albrecht M, Sharma CM, Reinhardt R, Vogel J, Rudel T: Deep sequencing-based discovery of the Chlamydia trachomatis transcriptome. Nucleic Acids Res. 2010, 38: 868-877.
Filiatrault MJ, Stodghill PV, Myers CR, Bronstein PA, Butcher BG, Lam H, Grills G, Schweitzer P, Wang W, Schneider DJ, Cartinhour SW: Genome-wide identification of transcriptional start sites in the plant pathogen Pseudomonas syringae pv. tomato str. DC3000. PLoS One. 2011, 6: e29335-
Perkins TT, Kingsley RA, Fookes MC, Gardner PP, James KD, Yu L, Assefa SA, He M, Croucher NJ, Pickard DJ, Maskell DJ, Parkhill J, Choudhary J, Thomson NR, Dougan G: A strand-specific RNA-Seq analysis of the transcriptome of the typhoid bacillus Salmonella typhi. PLoS Genet. 2009, 5: e1000569-
Kröger C, Dillon SC, Cameron ADS, Papenfort K, Sivasankaran SK, Hokamp K, Chao Y, Sittka A, Hébrard M, Händler K, Colgan A, Leekitcharoenphon P, Langridge GC, Lohan AJ, Loftus B, Lucchini S, Ussery DW, Dorman CJ, Thomson NR, Vogel J, Hinton JCD: The transcriptional landscape and small RNAs of Salmonella enterica serovar Typhimurium. Proc Natl Acad Sci USA. 2012, 109: E1277-E1286.
Wilms I, Overlöper A, Nowrousian M, Sharma CM, Narberhaus F: Deep sequencing uncovers numerous small RNAs on all four replicons of the plant pathogen Agrobacterium tumefaciens. RNA Biol. 2012, 9: 446-457.
Schlüter JP, Reinkensmeier J, Daschkey S, Evguenieva-Hackenberg E, Janssen S, Jänicke S, Becker JD, Giegerich R, Becker A: A genome-wide survey of sRNAs in the symbiotic nitrogen-fixing alpha-proteobacterium Sinorhizobium meliloti. BMC Genomics. 2010, 11: 245-
Batut J, Andersson SGE, O’Callaghan D: The evolution of chronic infection strategies in the α-proteobacteria. Nat Rev Microbiol. 2004, 2: 933-945.
Jones KM, Kobayashi H, Davies BW, Taga ME, Walker GC: How rhizobial symbionts invade plants: the Sinorhizobium-Medicago model. Nat Rev Microbiol. 2007, 5: 619-633.
Galibert F, Finan TM, Long SR, Pühler A, Abola P, Ampe F, Barloy-Hubler F, Barnett MJ, Becker A, Boistard P, Bothe G, Boutry M, Bowser L, Buhrmester J, Cadieu E, Capela D, Chain P, Cowie A, Davis RW, Dreano S, Federspiel NA, Fisher RF, Gloux S, Godrie T, Goffeau A, Golding B, Gouzy J, Gurjal M, Hernandez-Lucas I, Hong A, Huizar L, Hyman RW, Jones T, Kahn D, Kahn ML, Kalman S, Keating DH, Kiss E, Komp C, Lelaure V, Masuy D, Palm C, Peck MC, Pohl TM, Portetelle D, Purnelle B, Ramsperger U, Surzycki R, Thebault P, Vandenbol M, Vorhölter FJ, Weidner S, Wells DH, Wong K, Yeh KC, Batut J: The composite genome of the legume symbiont Sinorhizobium meliloti. Science. 2001, 293: 668-672.
Barnett MJ, Fisher RF, Jones T, Komp C, Abola AP, Barloy-Hubler F, Bowser L, Capela D, Galibert F, Gouzy J, Gurjal M, Hong A, Huizar L, Hyman RW, Kahn D, Kahn ML, Kalman S, Keating DH, Palm C, Peck MC, Surzycki R, Wells DH, Yeh KC, Davis RW, Federspiel NA, Long SR: Nucleotide sequence and predicted functions of the entire Sinorhizobium meliloti pSymA megaplasmid. Proc Natl Acad Sci USA. 2001, 98: 9883-9888.
Finan TM, Weidner S, Wong K, Buhrmester J, Chain P, Vorhölter FJ, Hernandez-Lucas I, Becker A, Cowie A, Gouzy J, Golding B, Pühler A: The complete sequence of the 1,683-kb pSymB megaplasmid from the N2-fixing endosymbiont Sinorhizobium meliloti. Proc Natl Acad Sci USA. 2001, 98: 9889-9894.
de Lucena DKC, Pühler A, Weidner S: The role of sigma factor RpoH1 in the pH stress response of Sinorhizobium meliloti. BMC Microbiol. 2010, 10: 265-
Ghosh T, Bose D, Zhang X: Mechanisms for activating bacterial RNA polymerase. FEMS Microbiol Rev. 2010, 34: 611-627.
Dombrecht B, Marchal K, Vanderleyden J, Michiels J: Prediction and overview of the RpoN-regulon in closely related species of the Rhizobiales. Genome Biol. 2002, 3: research0076-research0076.11
Oke V, Rushing BG, Fisher EJ, Moghadam-Tabrizi M, Long SR: Identification of the heat-shock sigma factor RpoH and a second RpoH-like protein in Sinorhizobium meliloti. Microbiology. 2001, 147: 2399-2408.
Sauviac L, Philippe H, Phok K, Bruand C: An extracytoplasmic function sigma factor acts as a general stress response regulator in Sinorhizobium meliloti. J Bacteriol. 2007, 189: 4204-4216.
Flechard M, Fontenelle C, Blanco C, Goude R, Ermel G, Trautwetter A: RpoE2 of Sinorhizobium meliloti is necessary for trehalose synthesis and growth in hyperosmotic media. Microbiology. 2010, 156: 1708-1718.
Fisher RF, Long SR: Rhizobium–plant signal exchange. Nature. 1992, 357: 655-660.
Marketon MM, Glenn SA, Eberhard A, González JE: Quorum sensing controls exopolysaccharide production in Sinorhizobium meliloti. J Bacteriol. 2003, 185: 325-331.
Hoang HH, Becker A, González JE: The LuxR homolog ExpR, in combination with the Sin quorum sensing system, plays a central role in Sinorhizobium meliloti gene expression. J Bacteriol. 2004, 186: 5460-5472.
Gurich N, González JE: Role of quorum sensing in Sinorhizobium meliloti-Alfalfa symbiosis. J Bacteriol. 2009, 191: 4372-4382.
Becker A, Barnett MJ, Capela D, Dondrup M, Kamp PB, Krol E, Linke B, Rüberg S, Runte K, Schroeder BK, Weidner S, Yurgel SN, Batut J, Long SR, Pühler A, Goesmann A: A portal for rhizobial genomes: RhizoGATE integrates a Sinorhizobium meliloti genome annotation update with postgenome data. J Biotechnol. 2009, 140: 45-50.
Krol E, Blom J, Winnebald J, Berhörster A, Barnett MJ, Goesmann A, Baumbach J, Becker A: RhizoRegNet–a database of rhizobial transcription factors and regulatory networks. J Biotechnol. 2011, 155: 127-134.
Mendoza-Vargas A, Olvera L, Olvera M, Grande R, Vega-Alvarado L, Taboada B, Jimenez-Jacinto V, Salgado H, Juárez K, Contreras-Moreira B, Huerta AM, Collado-Vides J, Morett E: Genome-wide identification of transcription start sites, promoters and transcription factor binding sites in E. coli. PLoS One. 2009, 4: e7526-
Buckstein MH, He J, Rubin H: Characterization of nucleotide pools as a function of physiological state in Escherichia coli. J Bacteriol. 2008, 190: 718-726.
Yuan ZC, Zaheer R, Finan TM: Regulation and properties of PstSCAB, a high-affinity, high-velocity phosphate transport system of Sinorhizobium meliloti. J Bacteriol. 2006, 188: 1089-1102.
Barnett MJ, Hung DY, Reisenauer A, Shapiro L, Long SR: A homolog of the CtrA cell cycle regulator is present and essential in Sinorhizobium meliloti. J Bacteriol. 2001, 183: 3204-3210.
Meyer F, Goesmann A, McHardy AC, Bartels D, Bekel T, Clausen J, Kalinowski J, Linke B, Rupp O, Giegerich R, Pühler A: GenDB–an open source genome annotation system for prokaryote genomes. Nucleic Acids Res. 2003, 31: 2187-2195.
Vesper O, Amitai S, Belitsky M, Byrgazov K, Kaberdina AC, Engelberg-Kulka H, Moll I: Selective translation of leaderless mRNAs by specialized ribosomes generated by MazF in Escherichia coli. Cell. 2011, 147: 147-157.
Sullivan MJ, Curson ARJ, Shearer N, Todd JD, Green RT, Johnston AWB: Unusual regulation of a leaderless operon involved in the catabolism of dimethylsulfoniopropionate in Rhodobacter sphaeroides. PLoS One. 2011, 6: e15972-
Krishnan KM, Etten WJV, Janssen GR: Proximity of the start codon to a leaderless mRNA’s 5′ terminus is a strong positive determinant of ribosome binding and expression in Escherichia coli. J Bacteriol. 2010, 192: 6482-6485.
Frank S, Klockgether J, Hagendorf P, Geffers R, Schöck U, Pohl T, Davenport CF, Tümmler B: Pseudomonas putida KT2440 genome update by cDNA sequencing and microarray transcriptomics. Environ Microbiol. 2011, 13: 1309-1326.
Brock JE, Pourshahian S, Giliberti J, Limbach PA, Janssen GR: Ribosomes bind leaderless mRNA in Escherichia coli through recognition of their 5′-terminal AUG.RNA. 2008, 14: 2159-2169.
O’Donnell SM, Janssen GR: The initiation codon affects ribosome binding and translational efficiency in Escherichia coli of cI mRNA with or without the 5′ untranslated leader. J Bacteriol. 2001, 183: 1277-1283.
Beaume M, Hernandez D, Farinelli L, Deluen C, Linder P, Gaspin C, Romby P, Schrenzel J, Francois P: Cartography of methicillin-resistant S. aureus transcripts: detection, orientation and temporal expression during growth phase and stress conditions. PLoS One. 2010, 5: e10725-
Filiatrault MJ, Stodghill PV, Bronstein PA, Moll S, Lindeberg M, Grills G, Schweitzer P, Wang W, Schroth GP, Luo S, Khrebtukova I, Yang Y, Thannhauser T, Butcher BG, Cartinhour S, Schneider DJ: Transcriptome analysis of Pseudomonas syringae identifies new genes, noncoding RNAs, and antisense activity. J Bacteriol. 2010, 192: 2359-2372.
Liu JM, Livny J, Lawrence MS, Kimball MD, Waldor MK, Camilli A: Experimental discovery of sRNAs in Vibrio cholerae by direct cloning, 5S/tRNA depletion and parallel sequencing. Nucleic Acids Res. 2009, 37: e46-
Andre G, Even S, Putzer H, Burguière P, Croux C, Danchin A, Martin-Verstraete I, Soutourina O: S-box and T-box riboswitches and antisense RNA control a sulfur metabolic operon of Clostridium acetobutylicum. Nucleic Acids Res. 2008, 36: 5955-5969.
Eiamphungporn W, Helmann JD: Extracytoplasmic function sigma factors regulate expression of the Bacillus subtilis yabE gene via a cis-acting antisense RNA. J Bacteriol. 2009, 191: 1101-1105.
Lee EJ, Groisman EA: An antisense RNA that governs the expression kinetics of a multifunctional virulence gene. Mol Microbiol. 2010, 76: 1020-1033.
Georg J, Voss B, Scholz I, Mitschke J, Wilde A, Hess WR: Evidence for a major role of antisense RNAs in cyanobacterial gene regulation. Mol Syst Biol. 2009, 5: 305-
Stazic D, Lindell D, Steglich C: Antisense RNA protects mRNA from RNase E degradation by RNA-RNA duplex formation during phage infection. Nucleic Acids Res. 2011, 39: 4890-4899.
Kawano M, Aravind L, Storz G: An antisense RNA controls synthesis of an SOS-induced toxin evolved from an antitoxin. Mol Microbiol. 2007, 64: 738-754.
Giangrossi M, Prosseda G, Tran CN, Brandi A, Colonna B, Falconi M: A novel antisense RNA regulates at transcriptional level the virulence gene icsA of Shigella flexneri. Nucleic Acids Res. 2010, 38: 3362-3375.
Silvaggi JM, Perkins JB, Losick R: Small untranslated RNA antitoxin in Bacillus subtilis. J Bacteriol. 2005, 187: 6641-6650.
Brantl S: Regulatory mechanisms employed by cis-encoded antisense RNAs. Curr Opin Microbiol. 2007, 10: 102-109.
Duehring U, Axmann IM, Hess WR, Wilde A: An internal antisense RNA regulates expression of the photosynthesis gene isiA. Proc Natl Acad Sci USA. 2006, 103: 7054-8.
Legewie S, Dienst D, Wilde A, Herzel H, Axmann IM: Small RNAs establish delays and temporal thresholds in gene expression. Biophys J. 2008, 95: 3232-3238.
Georg J, Hess WR: cis-antisense RNA, another level of gene regulation in bacteria. Microbiol Mol Biol Rev. 2011, 75: 286-300.
Reinkensmeier J, Schlüter JP, Giegerich R, Becker A: Conservation and occurrence of trans-encoded sRNAs in the Rhizobiales. Genes. 2011, 2: 925-956.
Barnett MJ, Bittner AN, Toman CJ, Oke V, Long SR: Dual RpoH sigma factors and transcriptional plasticity in a symbiotic bacterium. J Bacteriol. 2012, 194: 4983-4994.
Barnett MJ, Rushing BG, Fisher RF, Long SR: Transcription start sites for syrM and nodD3 flank an insertion sequence relic in Rhizobium meliloti. J Bacteriol. 1996, 178: 1782-1787.
Barnett MJ, Swanson JA, Long SR: Multiple genetic controls on Rhizobium meliloti syrA, a regulator of exopolysaccharide abundance. Genetics. 1998, 148: 19-32.
MacLellan SR, MacLean AM, Finan TM: Promoter prediction in the rhizobia. Microbiology. 2006, 152: 1751-1763.
Staroń A, Sofia HJ, Dietrich S, Ulrich LE, Liesegang H, Mascher T: The third pillar of bacterial signal transduction: classification of the extracytoplasmic function (ECF) σ factor protein family. Mol Microbiol. 2009, 74: 557-581.
Casse F, Boucher C, Julliot JS, Michel M, Dénarié J: Identification and characterization of large plasmids in Rhizobium meliloti using agarose-gel electrophoresis. J Gen Microbiol. 1979, 113: 229-242.
Barnett MJ, Long SR: S. meliloti strain differences. http://cmgm.stanford.edu/biology/long/strain_diffs,
Wecke T, Halang P, Staroń A, Dufour YS, Donohue TJ, Mascher T: Extracytoplasmic function σ factors of the widely distributed group ECF41 contain a fused regulatory domain. Microbiologyopen. 2012, 1: 194-213.
Nonaka G, Blankschien M, Herman C, Gross CA, Rhodius VA: Regulon and promoter analysis of the E. coli heat-shock factor, σ32, reveals a multifaceted cellular response to heat stress. Genes Dev. 2006, 20: 1776-1789.
Krol E, Becker A: Global transcriptional analysis of the phosphate starvation response in Sinorhizobium meliloti strains 1021 and 2011. Mol Genet Genomics. 2004, 272: 1-17.
Yuan ZC, Zaheer R, Morton R, Finan TM: Genome prediction of PhoB regulated promoters in Sinorhizobium meliloti and twelve proteobacteria. Nucleic Acids Res. 2006, 34: 2686-2697.
Blanco AG, Canals A, Bernués J, Solà M, Coll M: The structure of a transcription activation subcomplex reveals how σ70 is recruited to PhoB promoters. EMBO J. 2011, 30: 3776-3785.
Bardin SD, Voegele RT, Finan TM: Phosphate assimilation in Rhizobium (Sinorhizobium) meliloti: identification of a pit-like gene. J Bacteriol. 1998, 180: 4219-4226.
Laub MT, Chen SL, Shapiro L, McAdams HH: Genes directly controlled by CtrA, a master regulator of the Caulobacter cell cycle. Proc Natl Acad Sci USA. 2002, 99: 4632-4637.
Cheng J, Sibley CD, Zaheer R, Finan TM: A Sinorhizobium meliloti minE mutant has an altered morphology and exhibits defects in legume symbiosis. Microbiology. 2007, 153: 375-387.
Brilli M, Fondi M, Fani R, Mengoni A, Ferri L, Bazzicalupo M, Biondi EG: The diversity and evolution of cell cycle regulation in alpha-proteobacteria: a comparative genomic analysis. BMC Syst Biol. 2010, 4: 52-
Bellefontaine AF, Pierreux CE, Mertens P, Vandenhaute J, Letesson JJ, Bolle XD: Plasticity of a transcriptional regulation network among alpha-proteobacteria is supported by the identification of CtrA targets in Brucella abortus. Mol Microbiol. 2002, 43: 945-960.
Bailey TL, Williams N, Misleh C, Li WW: MEME: discovering and analyzing DNA and protein sequence motifs. Nucleic Acids Res. 2006, 34: W369-W373.
Barnett MJ, Toman CJ, Fisher RF, Long SR: A dual-genome Symbiosis Chip for coordinate study of signal exchange and development in a prokaryote-host interaction. Proc Natl Acad Sci USA. 2004, 101: 16636-16641.
Kazakov AE, Cipriano MJ, Novichkov PS, Minovitsky S, Vinogradov DV, Arkin A, Mironov AA, Gelfand MS, Dubchak I: RegTransBase–a database of regulatory sequences and interactions in a wide range of prokaryotic genomes. Nucleic Acids Res. 2007, 35: D407-D412.
Griffitts JS, Carlyon RE, Erickson JH, Moulton JL, Barnett MJ, Toman CJ, Long SR: A Sinorhizobium meliloti osmosensory two-component system required for cyclic glucan export and symbiosis. Mol Microbiol. 2008, 69: 479-490.
Carlyon RE, Ryther JL, VanYperen RD, Griffitts JS: FeuN, a novel modulator of two-component signalling identified in Sinorhizobium meliloti. Mol Microbiol. 2010, 77: 170-182.
Flechard M, Fontenelle C, Trautwetter A, Ermel G, Blanco C: Sinorhizobium meliloti rpoE2 is necessary for H2O2 stress resistance during the stationary growth phase. FEMS Microbiol Lett. 2009, 290: 25-31.
Staroń A, Mascher T: General stress response in α-proteobacteria: PhyR and beyond. Mol Microbiol. 2010, 78: 271-277.
Bastiat B, Sauviac L, Bruand C: Dual control of Sinorhizobium meliloti RpoE2 sigma factor activity by two PhyR-type two-component response regulators. J Bacteriol. 2010, 192: 2255-2265.
Meade HM, Long SR, Ruvkun GB, Brown SE, Ausubel FM: Physical and genetic characterization of symbiotic and auxotrophic mutants of Rhizobium meliloti induced by transposon Tn5 mutagenesis. J Bacteriol. 1982, 149: 114-122.
Glazebrook J, Walker GC: A novel exopolysaccharide can function in place of the calcofluor-binding exopolysaccharide in nodulation of alfalfa by Rhizobium meliloti. Cell. 1989, 56: 661-672.
Pellock BJ, Teplitski M, Boinay RP, Bauer WD, Walker GC: A LuxR homolog controls production of symbiotically active extracellular polysaccharide II by Sinorhizobium meliloti. J Bacteriol. 2002, 184: 5067-5076.
Schäfer A, Tauch A, Jäger W, Kalinowski J, Thierbach G, Pühler A: Small mobilizable multi-purpose cloning vectors derived from the Escherichia coli plasmids pK18 and pK19: selection of defined deletions in the chromosome of Corynebacterium glutamicum. Gene. 1994, 145: 69-73.
Sambrook J, Fritsch E, Maniatis E: Molecular cloning: A Laboratory Manual. 1989, New York: Cold Spring Harbor Laboratory Press
Beringer JE: R factor transfer in Rhizobium leguminosarum. J Gen Microbiol. 1974, 84: 188-198.
Vincent JM: A Manual for the Practical Study of Root Nodule Bacteria. IBP Handbook No. 15. 1970, Oxford: Blackwell Scientific Publications
Zhan HJ, Lee CC, Leigh JA: Induction of the second exopolysaccharide (EPSb) in Rhizobium meliloti SU47 by low phosphate concentrations. J Bacteriol. 1991, 173: 7391-7394.
Krol E, Becker A: ppGpp in Sinorhizobium meliloti: biosynthesis in response to sudden nutritional downshifts and modulation of the transcriptome. Mol Microbiol. 2011, 81: 1233-1254.
Hoffmann S, Otto C, Kurtz S, Sharma CM, Khaitovich P, Vogel J, Stadler PF, Hackermüller J: Fast mapping of short sequences with mismatches, insertions and deletions using index structures. PLoS Comput Biol. 2009, 5: e1000502-
Starmer J, Stomp A, Vouk M, Bitzer D: Predicting Shine-Dalgarno sequence locations exposes genome annotation errors. PLoS Comput Biol. 2006, 2: e57-
Barrios H, Valderrama B, Morett E: Compilation and analysis of σ54-dependent promoter sequences. Nucleic Acids Res. 1999, 27: 4305-4313.
Beckstette M, Homann R, Giegerich R, Kurtz S: Fast index based algorithms and software for matching position specific scoring matrices. BMC Bioinformatics. 2006, 7: 389-
Turatsinze JV, Thomas-Chollier M, Defrance M, van Helden J: Using RSAT to scan genome sequences for transcription factor binding sites and cis-regulatory modules. Nat Protoc. 2008, 3: 1578-1588.
Spencer W, Siam R, Ouimet MC, Bastedo DP, Marczynski GT: CtrA, a global response regulator, uses a distinct second category of weak DNA binding sites for cell cycle transcription control in Caulobacter crescentus. J Bacteriol. 2009, 191: 5458-5470.
Quandt J, Hynes MF: Versatile suicide vectors which allow direct selection for gene replacement in gram-negative bacteria. Gene. 1993, 127: 15-21.
Pinedo CA, Bringhurst RM, Gage DJ: Sinorhizobium meliloti mutants lacking phosphotransferase system enzyme HPr or EIIA are altered in diverse processes, including carbon metabolism, cobalt requirements, and succinoglycan production. J Bacteriol. 2008, 190: 2947-2956.
Edgar R, Domrachev M, Lash AE: Gene Expression Omnibus: NCBI gene expression and hybridization array data repository. Nucleic Acids Res. 2002, 30: 207-210.
This research was supported by German Research Foundation grants BE 2121/5-2 and GI 178/4-2 (SPP1258) to AB and RG, by the LOEWE program of the State of Hesse, Germany (in the framework of the Center for Synthetic Microbiology, SYNMIKRO, Marburg) to AB, and the Hoover Circle fund to SRL. MJB was supported by National Institutes of Health grant GM093628 to SRL. CL was supported by the German Academic Exchange Service (DAAD). We are grateful to Robert Fisher for construction of plasmid pF1084 and Esther Chen for critical reading of the manuscript.
The authors declare that they have no competing interests.
MJB, RG, SRL and AB designed the study. EK constructed the expR+ strain and provided the rpoE1 data. JPS carried out the experimental work for the RNAseq approach. JPS, JR, RG and AB formulated the RNAseq data analysis strategies. JR performed the bioinformatics analyses. MJB and CL did the Affymetrix GeneChip experiments and corresponding data analysis. MJB carried out the 5′ RACE mapping. All authors wrote the manuscript and approved the final version. All authors read and approved the final manuscript.
Jan-Philip Schlüter, Jan Reinkensmeier, Melanie J Barnett contributed equally to this work.
Electronic supplementary material
Additional file 2: Table S1: - TSS associated with tRNAs, repeat sequences, and transposable elements; Table S2- TSS associated with CDS, sRNAs, and asRNA; Table S3- Summary of newly identified and reannotated open reading frames; Table S4- Comparison of experimentally validated and predicted operons to transcription start site (TSS) data; Table S5- Comparison of RNAseq TSS to previously published TSS. (XLSX 2 MB)
Additional file 3: Table S6: - RpoD promoter sequences and their corresponding TSS; Table S7- RpoH1 promoter sequences and their corresponding TSS; Table S8- RpoH2 promoter sequences and their corresponding TSS; Table S9- Dual (RpoH1/H2) promoter sequences and their corresponding TSS; Table S10- RpoN promoter sequences and their corresponding TSS; Table S11- RpoE2 promoter sequences and their corresponding TSS; Table S12- RpoE1 promoter sequences and their corresponding TSS; Table S13- RpoE9 promoter sequences and their corresponding TSS. (XLSX 1 MB)
Additional file 4: Table S14: - Correlation of transcriptional regulator binding motifs with TSS; Table S15- Predicted CtrA binding motifs and their corresponding TSS; Table S16- Promoter motifs identified by MEME analyses; Table S17- Predicted FeuP binding motifs compared to TSS identified in this study and to microarray data for 14 feuP-dependent genes identified by Griffitts et al. . (XLSX 93 KB)
Additional file 5: Table S18: - Results of transcriptome analyses to identify putative RpoE2 target genes; Table S19- rpoE2-dependent genes with transcriptional activity correlated with TSS and promoter predictions; Table S20- rpoE2-dependent intergenic regions with transcriptional activity correlated with TSS and promoter predictions; Table S21- 5′ RACE mapping of TSS and comparison to RNAseq TSS; Table S22- Promoter-specific parameters used for promoter identification upstream of TSS; Table S23- Number of TSS assigned to each type of promoter sequence (virtual or model) used in the initial promoter search, by TSS category. (XLSX 150 KB)
About this article
Cite this article
Schlüter, J., Reinkensmeier, J., Barnett, M.J. et al. Global mapping of transcription start sites and promoter motifs in the symbiotic α-proteobacterium Sinorhizobium meliloti1021. BMC Genomics 14, 156 (2013) doi:10.1186/1471-2164-14-156
- Transcription start site
- Sigma factor
- Sinorhizobium meliloti
- Antisense RNA