Transcriptional regulation of the operon encoding stress-responsive ECF sigma factor SigH and its anti-sigma factor RshA, and control of its regulatory network in Corynebacterium glutamicum
© Busche et al.; licensee BioMed Central Ltd. 2012
Received: 9 February 2012
Accepted: 22 August 2012
Published: 3 September 2012
The expression of genes in Corynebacterium glutamicum, a Gram-positive non-pathogenic bacterium used mainly for the industrial production of amino acids, is regulated by seven different sigma factors of RNA polymerase, including the stress-responsive ECF-sigma factor SigH. The sigH gene is located in a gene cluster together with the rshA gene, putatively encoding an anti-sigma factor. The aim of this study was to analyze the transcriptional regulation of the sigH and rshA gene cluster and the effects of RshA on the SigH regulon, in order to refine the model describing the role of SigH and RshA during stress response.
Transcription analyses revealed that the sigH gene and rshA gene are cotranscribed from four sigH housekeeping promoters in C. glutamicum. In addition, a SigH-controlled rshA promoter was found to only drive the transcription of the rshA gene. To test the role of the putative anti-sigma factor gene rshA under normal growth conditions, a C. glutamicum rshA deletion strain was constructed and used for genome-wide transcription profiling with DNA microarrays. In total, 83 genes organized in 61 putative transcriptional units, including those previously detected using sigH mutant strains, exhibited increased transcript levels in the rshA deletion mutant compared to its parental strain. The genes encoding proteins related to disulphide stress response, heat stress proteins, components of the SOS-response to DNA damage and proteasome components were the most markedly upregulated gene groups. Altogether six SigH-dependent promoters upstream of the identified genes were determined by primer extension and a refined consensus promoter consisting of 45 original promoter sequences was constructed.
The rshA gene codes for an anti-sigma factor controlling the function of the stress-responsive sigma factor SigH in C. glutamicum. Transcription of rshA from a SigH-dependent promoter may serve to quickly shutdown the SigH-dependent stress response after the cells have overcome the stress condition. Here we propose a model of the regulation of oxidative and heat stress response including redox homeostasis by SigH, RshA and the thioredoxin system.
KeywordsCorynebacterium glutamicum ECF sigma factor Anti-sigma factor Promoter Microarray analysis
Corynebacterium glutamicum is a gram-positive, non-sporulating soil bacterium that belongs to the order Actinomycetales, which also includes genera like Mycobacterium and Streptomyces. C. glutamicum has been studied extensively because of its biotechnological application in the production of various amino acids. Besides this, it is of increasing importance as a model organism for other corynebacteria with biotechnological or medical significance, as well as for the species of related genera [1–3]. The data provided by the complete C. glutamicum genome sequence [4–6] enabled genome-wide analyses and the application of comparative genomics to assign functions to uncharacterized genes and to compare the genetic make-up with that of other bacterial species. Although the functions of the genes encoding transcriptional regulators or sigma factors of RNA polymerase may be assigned using comparative genomics, their role and connections in cell regulatory networks could hardly be deduced on the basis of genome sequences alone. Comparative transcriptome analyses of wild-type and mutant strains provide extensive sets of data enabling the connections between the nodes of the regulatory network to be determined.
Transcription initiation, in which an RNA polymerase (RNAP) holoenzyme plays the key role, is a major step in the regulation of bacterial gene expression. The RNAP core enzyme responsible for its catalytic activity consists of five subunits (α2ββ`ω) and associates with the σ subunit (factor), which is responsible for specific recognition of the promoter, to complete the fully functional RNAP holoenzyme. The majority of bacteria possess several sigma factors, which direct RNAP to different groups of promoters. The sigma factors thus form a specific class of regulators, which may affect the expression of large gene groups.
σ70-family sigma factors are categorized into four different classes . The essential (primary) group 1 sigma factors are responsible for the transcription of housekeeping genes, group 2 contains the primary-like sigma factors, group 3 sigma factors control genes involved in specific functions in some bacteria and group 4 sigma factors (also called ECF for extracytoplasmic function) are involved in responses to external stresses.
In C. glutamicum, SigA, the primary sigma factor (group 1), SigB, a primary-like sigma factor (group 2), and SigC, SigD, SigE, SigH and SigM, all of them ECF-type sigma factors, were found . SigB, SigE, SigH, and SigM are the only C. glutamicum sigma factors that have been studied so far. The genes included in their regulons were found to be involved in various stress responses [9–12].
Sigma factors are controlled by modulating their availability and activity. Anti-sigma factors bind to their cognate sigma factors in some cases, inhibiting their binding to the RNAP core enzyme. Controlling their activity by the reversible binding of an anti-sigma factor to the sigma factor in C. glutamicum was up to now only described for SigE by CseE . The activity of SigH or its orthologs is tightly controlled by anti-sigma factors in various actinobacteria. This has been demonstrated for M. tuberculosis RshA (a regulator of SigH) and S. coelicolor RsrA (a regulator of SigR, a SigH ortholog) that bind to their cognate sigma factors in a redox-responsive manner [11, 12]. Upon the oxidation of specific cysteine residues these anti-sigma factors change conformation, the respective bound sigma factor is released and can thus bind to RNAP, thereby activating its sigmulon (regulon of a sigma factor). After the cessation of the oxidative stress conditions, the reduced state is regenerated by the action of thioredoxins, and the anti-sigma factors regain their SigH-binding ability. The conserved cysteine residues have a conserved arrangement, the ZAS (zinc-containing anti-sigma factor) domain and the anti-sigma factors from different organisms can functionally replace each other .
It has been shown that C. glutamicum SigH is involved in responses to heat shock  and oxidative stress . The crucial role of SigH in the heat-shock response by controlling the expression of the ATP-dependent Clp protease, chaperones and heat-shock regulators was demonstrated in a number of studies [14–18]. The SigH-driven response to oxidative stress in actinobacteria generally includes the upregulation of the thioredoxin system (trxB and trxC) and at least one gene (mtr) of the mycothiol system, which are major antioxidant systems in these bacteria .
In addition to its involvement in the expression of a number of heat-shock response genes, C. glutamicum SigH was found to control the expression of genes encoding various stress regulators, such as HspR , ClgR , SufR , WhcA  and WhcE . Moreover, transcription of the genes encoding the sigma factors SigB and SigM is controlled by SigH [22–24]. Since SigH was found to be a major player in response to heat shock and oxidative stress, a regulatory network integrating the sigma factors SigH, SigB and SigM is apparently operative in C. glutamicum.
In this work, we demonstrate that the genes sigH and rshA, coding for the stress-responsive sigma factor and its putative anti-sigma factor, respectively, form an operon in C. glutamicum and are transcribed from multiple promoters of different classes. The SigH-dependent genes were defined on the basis of their enhanced transcription in the ΔrshA strain in the absence of environmental stimuli by DNA-microarray analysis and by q-RT-PCR. These results validated the assumption that RshA acts as an anti-SigH factor. We propose a model of the SigH-RshA regulatory network underlining the central role of SigH in the stress response of C. glutamicum.
The sigH gene and the rshA gene encoding an anti-sigma factor of SigH form an operon
In all C. glutamicum genomes, the translational stop codon of sigH is only separated by two bp from the translation initiation codon of rshA, indicating an operon-like structure. The deduced RshA protein sequence from C. glutamicum is only moderately similar to that of RshA from M. tuberculosis (35%) and RsrA from S. coelicolor (28%). An amino acid sequence alignment between the three corynebacterial genes and their M. tuberculosis and S. coelicolor counterparts (Additional file 1) shows that RshA from C. glutamicum carries the conserved cysteine residues which mediate the interaction of SigH and RshA in the ZAS domain .
The sigH gene and the rshA gene form an operon-like structure in C. glutamicum. We therefore first analyzed their transcriptional organization by Northern hybridization. The blotting was performed with total RNA prepared from C. glutamicum RES167 (restriction-deficient variant derived from the ATCC 13032 type strain and its derived deletion mutant strains DN2 (carrying a deletion within sigH) and AS1 (carrying a complete deletion of sigHrshA). The blot was then hybridized with DIG-labelled RNA-probes derived from the sigH and the rshA genes, respectively. A single 1-kb transcript hybridized with the sigH riboprobe when total RNA isolated from the RES167 strain was used (Figure 1b). A transcript of the same length also hybridized with the rshA riboprobe. These results indicated that both genes are transcribed in a single mRNA from a promoter located upstream of the sigH gene. An additional transcript of approximately 370 bp was detected by using the rshA riboprobe. This transcript most likely only covered the rshA gene and suggested that another promoter (PrshA) is present within the sigH coding region.
To address the question of whether the promoters of the sigH and rshA genes are controlled by the sigma factor SigH, we used RNA isolated from the sigH deletion strain DN2 for Northern hybridization. We supposed that the SigH- dependent transcripts would not be found with DN2 RNA. Indeed, no signal was detected when the sigH probe was used, because the complementary region in the sigH gene was deleted in DN2. A transcript of around 550 bp was detected with the rshA-specific probe (Figure 1b). This transcript most probably initiated upstream of sigH (from the sigH promoter), since its length was that of the full-length transcript containing sigH-rshA minus the length of the deletion within sigH in DN2 (Figure 1a). These results suggested that the bicistronic sigH-rshA transcript is formed in a SigH-independent manner. In contrast, the rshA transcript was not detected with the rshA probe, although the deletion within sigH should not have removed the presumed rshA promoter. This result indicated that the rshA promoter is under the control of SigH.
Genes of the sigH-rshA operon are transcribed from multiple promoters of different types
To analyze the promoter regions of the sigH-rshA operon and of the rshA gene, DNA fragments (504 bp upstream of sigH and 301 bp upstream of rshA) were cloned in the promoter probe vector pET2, thus forming transcriptional fusions of the promoter-active fragments and the reporter gene cat coding for chloramphenicol acetyltransferase (CAT). The activity of the promoters was measured using the CAT enzyme activity in cell-free extracts of C. glutamicum (pET2sigH) and C. glutamicum (pET2rshA). The activity of PsigH during the exponential growth phase was 0.1±0.015 U (mg of protein)-1 whereas the activity of PrshA was only 0.03 ±0.005 U (mg of protein)-1. Negligible activity was detected with the empty vector pET2 (≤0.003 U (mg of protein)-1). These measurements confirmed that rshA is also transcribed from the separate PrshA promoter.
Using total RNA from C. glutamicum (pET2rshA) and the CM4 primer, two TSPs were detected at nt G and A, 62 nt and 66 nt upstream of the rshA initiation codon (Figure 2d). TSP1 at the same G was detected by a weaker PEX result with the CM5 primer (not shown). The motifs TGGAAGA in the −35 region and TGTTAAA in the −10 region relative to TSP1 fit well to the consensus sequence of the −35 and −10 regions of the proposed SigH-dependent promoters of the M. tuberculosis (G/TGGAAC/TA −16 nt –C/GGTT)  and SigR-dependent promoters of S. coelicolor (GGGAA TG/C - 16 nt - C/GGTT G)  and also to the proposed C. glutamicum consensus of SigH-dependent promoters gGGAA ta - 16–19 nt - C/TGTT gaa  or G/TGGAA TA - 16–19 nt - C/TGTT GAA . This result suggests that the PrshA promoter is under the control of SigH, which is in agreement with the results from the Northern hybridization experiments.
Global transcriptional profiling of the rshA deletion mutant revealed the majority of known SigH-dependent genes and novel ones
Genes with enhanced expression in C. glutamicum Δ rshA compared with C . glutamicum RES167 (reference) sorted by function
Coding sequence a
Fold change b
Disulphide stress related genes
Alkanal monooxygenase (FMN-linked)
Putative dithiol-disulfide isomerase
Putative NADPH-dependent mycothiol reductase
Putative 1-D-myo-inosityl-2-amino-2-deoxy-alpha- D-glucopyranoside—L-cysteine ligase
Peptide methionine sulfoxide reductase
Putative dithiol-disulfide isomerase
Putative mycothiol S-conjugate amidase
Putative Fe-S-cluster redox enzyme
Transcriptional repressor of suf operon
quinone oxidoreductase involved in disulfide stress response
Heat stress-related genes
Chaperone, contains C-terminal Zn-finger domain
Endopeptidase Clp, proteolytic subunit
Putative ATP-dependent protease (heat-shock protein)
Endopeptidase Clp, proteolytic subunit
SOS and DNA repair genes
DNA/RNA helicase, superfamily I
Excinuclease ABC, ATPase subunit A
Putative RNA-binding protein
Putative methylated-DNA--protein-cysteine methyltransferase
Excinuclease subunit C
Putative proteasome component
prokaryotic ubiquitin-like protein
Trypsin-like serine protease
Genes with other function
Putative membrane protein
Conserved hypothetical protein
Putative multidrug efflux permease, MFS-type
Conserved hypothetical protein
Putative formate dehydrogenase, FdhD-family
tRNA (5-methylaminomethyl-2-thiouridylate) -methyltransferase
Putative phage-associated protein
Conserved hypothetical protein, HesB/YadR/YfhF family
Riboflavin synthase, alpha chain
Conserved hypothetical protein
Putative GTP cyclohydrolase II/3,4-dihydroxy-2-butanone-4-phosphatesynthase
ABC-type putative multidrug transporter, ATPase and permease subunit
Putative transcriptional regulatory protein
Riboflavin synthase, beta chain
Glucose-6-phosphate 1-dehydrogenase subunit
ABC-type ribose transporter, ATPase subunit (TC 3.A.1.2.1)
ABC-type ribose transporter, substrate-binding lipoprotein (TC 3.A.1.2.1)
ABC-type putative dipeptide/oligopeptide transporter, substrate-binding lipoprotein
Hypothetical protein, similar to ribosomal protein S2
Allophanate hydrolase subunit 2
Conserved hypothetical protein
ABC-type putative dipeptide/oligopeptide transporter, permease subunit
Putative monooxygenase, luciferase
ABC-type putative manganese/zinc transporter, ATPase subunit
Two-component system, sensory histidine kinase, putative pseudogene
ABC-type ribose transporter, permease subunit (TC 3.A.1.2.1)
Putative transcriptional regulatory protein
Putative Zn-dependent hydrolase
Conserved hypothetical protein
4-hydroxy-3-methylbut-2-en-1-yl diphosphate synthase
Putative secondary C4-dicarboxylate transporter, tripartite ATP-independent transporter (TRAP-T) family
ABC-type putative dipeptide/oligopeptide transporter, ATPase subunit
Putative membrane protein
Transcriptional repressor of ribose importer RbsACBD, LacI-family
Putative transcriptional regulator, HTH_3-family
Although most of the differentially transcribed genes match those described by Ehira et al., this study also found the genes mshC (cg1709; mycothiol synthesis) and mca (cg1127, mycothiol conjugate amidase) to be strongly deregulated, and qor2 (cg1553, quinone oxidoreductase) as weakly influenced in the ΔrshA mutant. All of these genes are apparently involved in redox homeostasis and were also found to be more strongly transcribed under disulphide stress conditions induced by diamide treatment (our unpublished results).
Interestingly, some heat-stress related genes previously reported to be SigH-dependent (dnaJ2, clpB, clpP1 and clpP2;[14, 16]) showed up only weakly in our analyses and some other previously identified members of the SigH regulon failed to exhibit the minimum threshold (m-value of 0.6 corresponding to 1.5-fold change) used. Genes that displayed differential expression values below this threshold were the dnaK-grpE operon, clpC, the non-essential sigma factor gene sigB and most genes of the suf cluster . A differential transcription of clgR, a heat stress-responsive regulator, which was expressed from a SigH-dependent promoter accoding to Engels et al., was also not detected in our experiments. This finding is similar to observations by Ehira et al.). These discrepancies might be explained by additional regulatory systems negatively controlling the transcription of these genes in the absence of (heat) stress.
Genes identified for the first time as being triggered by the SigH-RshA regulatory network included uvrA (cg1560) and uvrC (cg1790), both coding for subunits of the Exinuclease ABC (nucleotide-excision repair), as well as uvrD3 (cg1555), one of three genes encoding DNA helicases similar to UvrD proteins in C. glutamicum, and a gene cluster (cg0184-cg0186) possibly involved in alkylated DNA repair. Together with the observation of a putative LexA-regulated promoter upstream of the sigH-rshA operon, this links the SigH network with DNA damage and repair.
Other newly identified genes code for components of the proteasome machinery, pup (cg1689; encoding a prokaryotic ubiquitin-like protein) and cg0998 (a trypsin-like serine protease). All these genes were found to be transcriptionally induced in the ΔrshA strain (Table 1).
Among the downregulated genes, only 7 exceeded the standard threshold m < −1 (fold change 0.5). These genes encode putative membrane proteins, hypothetical proteins and transporters (Additional file 2). Interestingly, the sigH transcript itself appeared to be less abundant in the rshA deletion mutant. Since this result was unexpected, we checked PsigH for mutations in this strain by PCR amplification and sequencing of the sigH 5’-upstream region. No mutations were found within 315 bp upstream of the sigH translational start codon (data not shown). It can be speculated that the sigH transcript is less stable in the ΔrshA mutant due to a change in its structure or due to the lack of stablisation effects by ribosomes translating rshA.
To validate the newly found potential SigH-dependent genes, we focussed our subsequent analyses on those from which new insights into the SigH regulon were expected. Therefore the genes potentially involved in response to disulphide stress, in protein degradation and in SOS response to DNA damage were included in the following q-RT-PCR experiments.
Differential transcription of selected SigH-dependent genes was validated by quantitative real-time RT-PCR
The microarray analyses found a number of novel candidate genes for the SigH regulon. To validate these results, we performed a q-RT-PCR with mshC, mca and mtr (involved in mycothiol synthesis and recycling [30, 31]), pup (encoding an ortholog of the recently identified prokaryotic ubiquitin-like protein in M. tuberculosis), as well as uvrA and uvrD3 (SOS-response). Additionally, we chose the two genes with strongly enhanced expression in the ΔrshA strain, cg2838 (putative dithiol-disulfide isomerase) and cg3405 (NADPH:quinone reductase), which might be involved in defense against disulphide stress. The recently described small antisense RNA arnA that has been shown to be transcribed from a SigH-dependent, heat-shock-induced promoter  was also included in the q-RT-PCR analysis. The arnA transcript was not addressed in the microarray analysis, since only probes for protein-coding genes were used in the design of the microarray .
Experimental localization of SigH-dependent promoters and derivation of a consensus sequence
The sigH-rshA operon in C. glutamicum exhibits complex transcriptional organization including autoregulation
In this study we demonstrated the upregulation of the majority of the known SigH-dependent genes in the absence of an applied stress by removing its putative anti-sigma factor RshA. The gene encoding RshA was only annotated in the genome of C. glutamicum ATCC 13032, reported by Kalinowski et al.. The rshA gene in two other sequenced C. glutamicum strains, in C. glutamicum ATCC 13032, reported by Ikeda and Nakagawa , and C. glutamicum strain R, reported by Yukawa et al., is not annotated, probably because of its small size of 89 amino acids. However, the deduced RshA protein sequences are identical in the three genome sequences and similar to other anti-sigma factors from M. tuberculosis (RshA; ) or S. coelicolor (RsrA; ). RshA from C. glutamicum shares the conserved cysteine residues in the ZAS domain with its counterparts. These residues modulate the interaction with the SigH protein, a fact that has been experimentally determined for RshA and SigH in M. tuberculosis, RsrA and SigR in S. coelicolor, as well as for other members of the ZAS-domain containing protein family in actinobacteria . The clear upregulation of all previously determined SigH-dependent genes in the constructed rshA mutant provides further proof that in C. glutamicum, RshA functions as an anti-sigma factor similar to M. tuberculosis RshA and S. coelicolor RsrA.
The sigH-rshA gene organization is also conserved in all sequenced Corynebacterium strains available in NCBI database e.g. C. glutamicum, C. efficiens, C. jeikum, and in the more distantly related S. coelicolor. M. tuberculosis exhibits a similar organization, but a gene encoding a protein of unknown function is inserted between the sigH and rshA genes.
The transcriptional organization of the sigH-rshA operon in C. glutamicum is similar but not identical to that of M. tuberculosis and S. coelicolor. In C. glutamicum, four promoters upstream of sigH-rshA resemble house-keeping promoters which are recognized by SigA. The reason for having multiple promoters might ensure fine-tuning, either by the action of additional transcription factors or by the differing affinities of these promoters to SigA and SigB, the non-essential sigma factor of C. glutamicum that also targets house-keeping promoters . Experimental observations are in line with this assumption: it was shown by a reporter fusion analysis (P-sigH::cat) that the activity of the sigH promoter rose in the stationary phase and after oxidative stress , whereas no significant changes in sigH transcript levels were detected after heat shock  or in the transition phase of growth . In S. coelicolor, the sigR-rsrA operon is also transcribed from multiple promoters. There is one transcriptional start of sigR dependent on the housekeeping sigma factor SigA and another one dependent on SigRSc itself . In M. tuberculosis, sigH is apparently only autoregulated by SigH .
A possible additional regulation of SigH in C. glutamicum might operate via the SigA-dependent promoter that was found in the 5´-UTR of the sigH gene, overlapping with a putative SOS-box  and therefore most likely blocked by the LexA repressor in the absence of a DNA-damaging agent.
The main difference from the related bacteria S. coelicolor and M. tuberculosis was the finding that in C. glutamicum, the rshA gene is transcribed by an additional promoter as a monocistronic transcript. We showed by Northern blotting and by PEX analysis that this transcription is SigH-dependent. It can be speculated that this transcriptional organization evolved to guarantee an excess of RshA protein over SigH at all times and therefore a fast shut-down of SigH-dependent transcriptional activation as soon as stress conditions end.
Expression analysis of the rshA mutant strain validated and extended the known SigH regulatory network
Genes hitherto not described as being part of the SigH regulon included genes involved in mycothiol (MSH) synthesis and recycling. Besides thioredoxin (Trx), MSH is the major low-molecular mass thiol in corynebacteria, mycobacteria and streptomycetes . The biosynthesis of MSH in C. glutamicum and two essential genes, mshC and mshD involved in the biosynthetic pathway have been described . In our approach, we observed a SigH-dependent upregulation of mshC, coding for the second gene in mycothiol (MSH) synthesis, and mca as well as mtr, involved in mycothiol recycling (Figure 8).
Mca is the first gene in MSH recycling and was already shown to be transcribed in a SigH-dependent manner . It encodes mycothiol S-conjugate amidase (Mca), which cleaves adducts (MSR) from the reaction of MSH with electrophiles to produce a mercapturic acid (AcCySR) and 1-O-(2-amino-2-deoxy-a-D-glucopyranosyl)-D-myo-inositol (GlcN-Ins) [30, 31]. GlcN-Ins is the substrate of MshC, and MSH is synthesized from the subsequent enzymatic reaction with MshD . As was mentioned above, mshD was not observed to be transcribed in a SigH-dependent manner, but its transcription was induced by disulphide treatment in C. glutamicum (our unpublished results), indicating that mshD is transcriptionally regulated. In M. tuberculosis, all the genes of MSH synthesis seem to be transcribed constitutively . There is a similar mechanism in S. coelicolor, with the difference that besides mca, mshA is transcriptionally induced as a direct target of SigR and the genes mshB, mshC and mshD are SigR-dependent, but apparently induced indirectly .
The SOS regulon of many bacteria, including E. coli, is involved in various cellular processes, e.g. nucleotide excision and recombination repair . By deleting the gene encoding the SOS response regulator LexA in C. glutamicum, Jochmann and coworkers  defined the SOS response in C. glutamicum, with only one of the uvr genes, namely uvrC, showing up in the microarray as differentially transcribed.
In our approach we observed a SigH-dependent induction of three uvr genes (uvrA, uvrC, uvrD3). The induction of uvrC transcription was quite low in our experiments, most likely because of an additional repression by LexA. As mentioned in , the degree of induction of SOS gene expression depends on at least four parameters: (i) the affinity of LexA for the SOS box, (ii) the location of the SOS box relative to the promoter, (iii) the promoter strength, and (iv) the presence of any additional constitutive promoters [39–41]. In this context, it is apparent that SigH is involved in the SOS response in C. glutamicum, integrating it with the heat stress and thiol-oxidative stress defense systems into a general stress response network.
This is in accordance with a proposal made by Barreiro et al.. The regulation of sigH in cases of severe stress (probably causing DNA damage) would release LexA from the SOS boxes and thereby activate an additional SigA-dependent sigH promoter.
The SigH regulatory network appears to also control other functions. An interesting novel finding was the enhanced transcription of components of the proteasome. The actinobacterial proteasome consists of functions for pupylation (a process similar to eukaryotic ubiquitinylation, which marks proteins that are to be degraded) and proteases. Our study connects the recently identified pupylation component Pup (prokaryotic ubiquitin-like protein) and PafA2 (proteasome acessory factor, responsible for Pup conjugation; ) with the SigH regulon and underlines that SigH also plays a significant role in protein quality control.
Based on the results obtained in this study and in previous studies, we propose an extended model of the SigH regulon in C. glutamicum (Figure 8) including the direct control of the stress reponse to disulphide and heat stress by RshA, involving the thioredoxin system and the mycothiol-recycling system to cope with thiol-depleting conditions. In an unstressed state, SigH is inhibited by the reduced form of RshA. The disruption of the SigH–RshA complex in C. glutamicum appears under severe heat shock or disulphide stress via a change in the conformation through the oxidation of RshA. The released SigH forms a functional RNAP holoenzyme with the core enzyme and induces the stress response by transcribing SigH-dependent genes, including those involved in disulphide and heat stress response. The feed-forward induction of the anti-sigma factor RshA enables the cell to quickly shut down the stress response, based on SigH-dependent transcription, after the stress ends. RshA, as the stress-sensing redox switch, is one of the targets of the biochemical pathways encoded by genes of the SigH network, namely those of the reducing compounds thioredoxin (Trx) and mycothiol (MSH). Direct induction of trxB1C generates the thiol Trx and the gene products of trxB, mtr, mca, and mshC reduce and/or recycle Trx and MSH, respectively, which are able to restore, together with other reductases and reducing compounds, the thiol redox balance and reverse the oxidation of cysteine residues in RsrA. In this closed loop, RshA is reduced to regain its functionality and binds SigH after redox homeostasis is reached. A similar model was developed for the thiol-depleting stress response in S. coelicolor by Newton and coworkers in 2008 [30, 31]. The transcriptional regulatory network controlled by SigH is highly connected to other regulators, modulating gene expression in response to other physical or chemical triggers. The heat-shock regulatory network that includes the regulators HspR and ClgR is an example of such a level of control.
In this study, we approached the SigH regulatory network in C. glutamicum from another angle. In the absence of stress, the SigH regulon was induced by removing its cognate anti-sigma factor RshA. Our findings on the regulatory network on the one hand extended the known functions controlled by SigH, and on the other hand demonstrated that stress most likely imposes further actions that modulate the transcriptional control of apparently stress-related or unrelated genes. In the end, sigma factor competition at the RNAP determines whether an effect on the transcription of a certain gene is exerted as well as how strong it will be. In addition, factors like RNA degradation and proteolysis will surely have significant influences on all aspects of the network. Hence, a considerable amount of work lies ahead before we can claim that a single sigma factor network in C. glutamicum is understood.
Bacterial strains, plasmids, oligonucleotide primers, media and growth conditions
Plasmids and bacteria used in this work
sacB, lacZ α, mcs (KmR)
E. coli–C. glutamicum promoter-probe vector (KmR, promoterless cat gene)
sigH promoter region (550 bp) in pET2
rshA promoter region (301) in pET2
P4sigH promoter region (348 bp) in pET2
E. coli JM109
end A1, rec A1, gyr A96, thi, hsd R17 (rk–, mk+), rel A1, sup E44, Δ(lac-proAB), F´ tra D36, proAB, laqI q lacZ ΔM15
restriction-deficient C. glutamicum strain ( ΔcglIM-cglIR-cglIIR)
RES167 deletion of sigH
RES167 deletion of sigH-rshA
RES167 deletion of rshA
DNA isolation, manipulation and transfer
Isolation of plasmid DNA from E. coli cells by an alkaline lysis technique was performed using a QIAprep Spin Miniprep Kit (Qiagen, Hilden, Germany). Chromosomal C. glutamicum DNA was isolated as described previously . DNA amplification by PCR was carried out with KOD DNA polymerase (Merck, Darmstadt, Germany) or Phusion DNA polymerase (Finnzymes,Vantaa, Finland) and chromosomal C. glutamicum RES167 DNA as the template. PCR products were purified with a QIAquick PCR Purification Kit (Qiagen). All oligonucleotides used in this study (Additional file 1) were purchased from Metabion (Martinsried, Germany). All PCR setups were done according to the manufacturers´ protocols. Modification of DNA, analysis by agarose gel electrophoresis and ligation were performed using standard procedures . E. coli was transformed with plasmid DNA using the method of Hanahan , C. glutamicum cells were transformed by electroporation [46, 47].
Construction of defined deletions in the C. glutamicum chromosome
The defined chromosomal deletions (ΔrshA, ΔsigH and ΔsigHrshA) were constructed in C. glutamicum RES167 using the gene SOEing procedure , the E. coli vector pK18mobsacB and the conditional lethal effect of the sacB gene for selecting double recombinants after the transformation of C. glutamicum. The selection of the resulting marker-less C. glutamicum strains ΔrshA, DN2 and AS1 and PCR confimation of the respective rshA (220 bp) sigH (450 bp) and sigHrshA (1340 bp) deletions within their chromosomes (Figure 1A) were carried out as described previously  using the primers listed in the Additional file 3.
Construction of plasmids
Fragments carrying the promoter regions of the genes sigH, sigH(P4), rshA, mshC, mca, dnaJ2 uvrA and uvrD were amplified from the chromosomal DNA of C. glutamicum by PCR with the primer pairs PSIGHF+PSIGHR, PSIGHF+PSIGH4R, PRSHAF+PRSHAR, PMSHCF+PMSHCR, PMCAF+PMCAR, PDNAJ2F+PDNAJ2R, PUVRAF+PUVRAR and PUVRDF+PUVRDR, respectively (Additional file 3). The primers carried the PstI, BamHI or BglII restriction sites. The PCR products were digested by the respective enzymes and cloned in the plasmid pET2 digested by PstI and BamHI. The resulting plasmid constructs were introduced into C. glutamicum by electroporation.
RNA isolation and quantitative real-time RT-PCR
RNA was isolated from exponentially growing cultures of both C. glutamicum RES167 and the ΔrshA strain grown in triplicate. The cells were harvested by centrifugation and the cell pellets were immediately frozen in liquid nitrogen. The cells were then resuspended in the RLT buffer provided with the RNeasy Mini Kit (Qiagen, Hilden, Germany) and disrupted with a Precellys 24 homogeniser (Bertin Technologies, France) at a speed of 6.5 for 30 s once.
Total RNA was purified with an RNeasy Mini Kit along with an RNase-Free DNase Set (Qiagen) and a DNase I Kit (Sigma-Aldrich, Taufkirchen, Germany) according to a previously published protocol . RNA was quantified with a NanoDrop ND-1000 spectrophotometer (Thermo Scientific, Wilmington, DE). Purified total RNA from C. glutamicum cultures was used in real time RT-PCR analysis performed with a LightCycler instrument (Roche Diagnostics, Mannheim, Germany) and a 2× SensiMix One Step Kit (Bioline, Luckenwalde, Germany). The verification of the resulting RT-PCR products was performed by melting curve analysis. The differences in gene expression were determined by comparing the crossing points of three samples measured in duplicate. The crossing points were determined using the LightCycler software (Roche Diagnostics). The calculation of the average crossing point (CP) was performed by first calculating the averages for each set of technical replicates and then by calculating the average of the three biological replicates. For each set of three biological replicates, the standard deviation was calculated (assuming a normal distribution of the CPs) and the combined standard deviation for the DeltaCP was approximated using the standard calculation for the propagation of uncertainity (assuming non-correlated errors).
The hybridization of whole-genome oligonucleotide microarrays was performed as described previously , using 8 μg of total RNA from C. glutamicum cultures for cDNA synthesis. The normalization and evaluation of the hybridization data was done with the software package EMMA 2  using a signal intensity (A-value) cut-off of ≥7.0 and a signal intensity ratio (M-value) cut-off of ±0.6, which corresponds to relative expression changes equal to or greater than 1.5-fold.
Northern blot analysis
The DIG-labeled RNA probes for the sigH and rshA genes for transcript analysis were obtained by in vitro-transcription with T7 RNA polymerase, NTP-DIG-label mix (Roche Diagnostics) and gene-specific primers with a T7 promoter-sequence attached to the reverse primer (Additional file 3). Prior to hybridization, the probes were denatured by incubation at 95°C for 10 min.
Northern blot analysis was performed as described by Homuth et al. with the following modifications. Total RNA samples (5 μg), purified by using the RNeasy Mini Kit along with the RNase-Free DNase Set (Qiagen) and the DNase I Kit (Sigma-Aldrich) according to a previously published protocol , were separated under denaturing conditions in 1% agarose-formaldehyde gels in 1xMOPS (morpholinepropanesulfonic acid) running buffer and stained with ethidium bromide. Separated RNA was transferred to a Hybond-N membrane (GE Healthcare, Freiburg, Germany) by vacuum blotting. Hybridization and detection were carried out as follows. After being baked at 120°C for 0.5 h, the membrane was prehybridized under stringent conditions at 68°C for 1 h in 50% formamide and 5x SSC (1x SSC is 0.15 M NaCl plus 0.015 M sodium citrate) without the probe to block reactive membrane binding sites, and in the second step hybridized with digoxigenin (DIG)-labelled RNA probes (50 ng/ml) at 68°C overnight. The hybridized membrane was washed to remove the hybridization solution, first twice for 10 min in 2× SSC-0.1% (wt/vol) sodium dodecyl sulfate (SDS) at room temperature and then three times for 15 min in 0.1× SSC-0.1% (wt/vol) SDS at 68°C, and hybridization signals were detected according to the manufacturer’s instructions (Roche Anti-Digoxigenin-AP, Fab fragments 2 μl and CDP-Star) with a Luminescent Image Analyzer LAS-3000 (Fujifilm Europe, Düsseldorf, Germany). The sizes of the detected signals were determined by comparing with the prior ethidium-bromide-stained High Range Marker (Fermentas, St. Leon-Roth, Germany), marked on the membrane.
Primer extension analysis
C. glutamicum cells were cultivated in 2xTY medium at 30°C, harvested at OD600 = 3.5, and frozen at −70°C. The pellet was resuspended in distilled water and approximately 0.2 × 108 cells were disintegrated with a FastPrep FP120 (BIO101) (6x20 s, speed 6.0) using glass beads. The suspension was cooled for 5 min on ice between runs. The cell debris was removed by centrifugation and total RNA was isolated from the extract using a High Pure RNA Isolation Kit (Roche Diagnostics). The primer extension analysis was essentially done as described previously . Reverse transcription was performed with SuperScript III transcriptase (Invitrogen, Carlsbad, CA) using 30 μg RNA and 5 pmol Cy-5-labeled primer CM4 or CM5 (Additional file 3) complementary to the vector pET2. Specific Cy5-labeled primers XMSHC, XMCA and XUVRD (Additional file 3) were used to determine the transcriptional start points of the genes mshC, mca and uvrD, respectively. PAA gel electrophoresis was run with the synthesized cDNA simultaneously with the DNA sequencing products generated with the same labeled primer in an A.L.F. Sequencer (GE Healthcare, Munich, Germany).
Chloramphenicol acetyltransferase (CAT) assay
The CAT activity was essentially measured as described previously . C. glutamicum strains harboring the vector pET2 with promoter-carrying fragments were cultivated in complete 2xTY medium to OD600 = 3 to 3.5. The cells were rapidly chilled on ice and disrupted with a FastPrep FP120 homogenizer (BIO101) (Thermo Scientific). The specific CAT activity in the cell-free extracts was determined photometrically at 412 nm as described by Shaw . One unit (U) of enzyme activity was defined as 1 μmol of chloramphenicol acetylated per minute.
Acknowledgements and funding
The authors wish to thank J. Nešvera for critical reading of the manuscript. This work was supported by grant Ka1722/1-1 from the Deutsche Forschungsgemeinschaft (DFG) and by Grant 204/09/J015 from the Scientific Council of the Czech Republic and by Institutional Research Concept No. AV0Z50200510.
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