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  • Research article
  • Open Access

Transcriptional cross-activation between toxin-antitoxin systems of Escherichia coli

BMC Microbiology201313:45

https://doi.org/10.1186/1471-2180-13-45

©  Kasari et al; licensee BioMed Central Ltd. 2013

  • Received: 13 December 2012
  • Accepted: 18 February 2013
  • Published:

Abstract

Background

Bacterial toxin-antitoxin (TA) systems are formed by potent regulatory or suicide factors (toxins) and their short-lived inhibitors (antitoxins). Antitoxins are DNA-binding proteins and auto-repress transcription of TA operons. Transcription of multiple TA operons is activated in temporarily non-growing persister cells that can resist killing by antibiotics. Consequently, the antitoxin levels of persisters must have been dropped and toxins are released of inhibition.

Results

Here, we describe transcriptional cross-activation between different TA systems of Escherichia coli. We find that the chromosomal relBEF operon is activated in response to production of the toxins MazF, MqsR, HicA, and HipA. Expression of the RelE toxin in turn induces transcription of several TA operons. We show that induction of mazEF during amino acid starvation depends on relBE and does not occur in a relBEF deletion mutant. Induction of TA operons has been previously shown to depend on Lon protease which is activated by polyphospate accumulation. We show that transcriptional cross-activation occurs also in strains deficient for Lon, ClpP, and HslV proteases and polyphosphate kinase. Furthermore, we find that toxins cleave the TA mRNA in vivo, which is followed by degradation of the antitoxin-encoding fragments and selective accumulation of the toxin-encoding regions. We show that these accumulating fragments can be translated to produce more toxin.

Conclusion

Transcriptional activation followed by cleavage of the mRNA and disproportionate production of the toxin constitutes a possible positive feedback loop, which can fire other TA systems and cause bistable growth heterogeneity. Cross-interacting TA systems have a potential to form a complex network of mutually activating regulators in bacteria.

Keywords

  • Toxin-antitoxin systems
  • Transcriptional regulation
  • Regulatory network
  • mRNA stability
  • Persisters

Background

Bacterial toxin-antitoxin (TA) systems are complexes of a stable toxic- or growth-arresting factor and its unstable inhibitor [1, 2]. They are diverse, abundant in all bacteria, except a few intracellular parasites, and are found in many archaea [3–6]. On the basis of their ubiquity and diversity, we can assume that regulation by TA must be common and beneficial in a wide range of microorganisms. However, their role in bacterial physiology is unclear [7, 8], in part due to redundancy [9]. They were first discovered in plasmids and characterized as addiction systems, which are responsible for post-segregational killing [10]. However, because of its high cost to the host, such a stability mechanism is used only in rare cases [11]. Chromosomal TA loci were found thanks to full genome sequencing [4] and were demonstrated to be functional, expressed at significant levels, and activated by various stressful conditions, particularly by amino acid starvation [12–15].

Our current study focuses on type II TA systems. In this group, both the toxin and the antitoxin are proteins, which are encoded by adjacent co-transcribed genes. In a growing cell, toxins are neutralized by tightly bound antitoxins. Antitoxins are degraded by proteases much more quickly than toxins, and if antitoxin production stops, toxins target vital functions of the producer through diverse mechanisms. Many toxins (e. g. RelE, MazF, YafQ, HigB, HicA, MqsR) are endoribonucleases and inhibit protein synthesis through cleavage of free or ribosome-bound mRNA [16–21]. MazF also cleaves 16S rRNA [22] and VapC endonucleases of enteric bacteria cleave initiator tRNA [23]. Another group of toxins (CcdB, ParE) interferes with DNA gyrase [24, 25], whereas HipA is a protein kinase [26, 27], and zeta toxins (PezT) inhibit cell wall synthesis [28]. Activation of toxins causes growth inhibition and dormancy that may be transient [29] but in some circumstances is irreversible and leads to cell death [28, 30–32].

Besides direct protein-protein interaction, antitoxins regulate toxin activity at the level of transcription. Antitoxins are DNA-binding proteins and specifically repress transcription of their own TA operons both alone and, even more effectively, in complexes with their cognate toxins. Degradation of an antitoxin causes de-repression of the TA promoter [33] and allows the toxin activity to be detected indirectly by measurement of transcript levels. Gerdes and colleagues have demonstrated fine-tuning of transcription by the toxin:antitoxin ratio for the RelBE system [34, 35]. The RelB antitoxin in excess of the RelE toxin promotes formation of the RelB:RelE (2:1) complexes that bind to the operator sites and repress transcription. RelE toxin in excess promotes formation of the ReB:RelE (2:2) complexes that are unable to bind DNA [36]. As a result, over-expression of RelE causes substantial increase in the relBE mRNA level. These authors suggested that such transcriptional regulation by the T:A ratio is commonplace for TA loci [35] and demonstrated it recently for VapBC [37]. Importantly, the levels of TA mRNAs were increased in cell populations enriched for persisters, thereby linking TA systems to antibiotic susceptibility [38, 39]. Persisters are transiently dormant bacteria that remain non-dividing under growth-supporting conditions and are not killed by bactericidal antibiotics [40]. TA systems, by their very nature, may be primarily responsible for persister formation. Mutations that increase toxicity of the TA toxins were shown to increase the frequency of persisters and cause high persistence phenotypes [41, 42]; and deletion of the yafQ toxin significantly decreased persister frequency in E. coli biofilms [43]. A recent study reports that successive deletion of 10 endoribonuclease-encoding TA loci progressively reduced the level of persisters while single deletions of TA systems had no effect on persister frequency in planktonic E. coli[44]. Hence, it is extremely important to consider redundancy and possible cross-talk when we study TA-related phenotypes, because most bacterial genomes contain multiple TA loci.

In the current study we found that uninhibited toxins can activate transcription of the other TA operons. Cleavage of these transcripts by endoribonuclease toxins adds another layer of complexity. Reciprocal transcriptional de-repression and transcript cleavage predict that toxin-antitoxin systems have a potential to form a complex network of regulators that controls growth and dormancy of bacteria.

Results

Uninhibited toxins can activate other toxin-antitoxin systems

Excess of a toxin has been shown to destabilize binding of the toxin-antitoxin complex to operator DNA and to activate transcription of its own operon [35]. To test whether toxins can activate transcription of other TA operons, we measured the transcription of relBE in response to ectopic expression of toxins MazF, MqsR, YafQ, HicA, and HipA by northern hybridization (Figure 1). Since the relBE genes are co-transcribed with the downstream relF[45], which encodes a hok-like toxin targeted against the inner membrane [46], we analyzed the transcription of the full relBEF operon. In a reverse experiment, we over-expressed RelE and monitored the transcription of several chromosomal TA operons (Figure 2). Amino acid starvation is known to upregulate relBEF transcription [14] and was induced by addition of mupirocin (MUP) [47] as a positive control. Ectopic expression of RelE served as an additional positive control for activation of relBEF transcription whereas synonymous substitutions were introduced into the plasmidal relE sequence (Additional file 1: Table S2; primer relE-XbaUP) to enable unambiguous detection of the chromosomal relE transcript. Active RelE toxin could be expressed from the altered gene (Additional file 1: Figure S1) and the plasmidal transcript was not detectable in the ΔrelBEF strain, showing that our hybridization probes are specific and do not cross-hybridize (Additional file 1: Figure S3A,B,C lanes 1,2). Toxins were induced in log phase cultures and concomitant measurements of optical density confirmed growth inhibition in all cultures tested (Additional file 1: Figure S1). Samples for RNA isolation were collected before induction (−1 min) and during a two hour time-course post-induction (15, 60 and 120 min); mRNA of the chromosomal TA operon was analyzed by northern hybridization using DNA oligoprobes complementary to relB, relE, and relF (Figure 1; Additional file 1: Table S2).
Figure 1
Figure 1

Northern analysis of relBEF transcription in response to expression of different toxins. Cultures of BW25113 contained plasmids for toxin and antitoxin expression. Toxins were induced and RNA was extracted at timepoints −1(before induction), 15, 60, and 120 min; 10-μg aliquots were subjected to electrophoresis, transferred to a membrane, and hybridized with oligoprobes relB (A), relE (B), and relF (C). Localization of the hybridization probes is shown on the map of the relBEF operon and the full-length relBEF transcript is marked by arrowhead (◄). Cultures of toxin over-expression contained the following plasmids: RelE - pVK11; MazF - pSC3326 and pSC228; MqsR - pTX3 and pAT3; YafQ - pBAD-yafQ and pUHE-dinJ; HicA - pMJ221 and pMJ331; HipA - pNK11 and pNK12. Control cultures contained the empty vectors pBAD33 and pOU82. Mupirocin (MUP) was added as a positive control for transcriptional activation of relBEF.

Figure 2
Figure 2

Transcription of TA operons in response to expression of RelE. Production of RelE was induced in cultures of BW25113 bearing plasmids pKP3035 and pKP3033. RNA extracted at timepoints −1 (before induction), 15, 60, and 120 min was subjected to northern analysis using oligoprobes complementary to the mRNAs of different toxins (underlined) and antitoxins. Panel A refers to the first and panel B to the second gene of the TA operon.

As shown in Figure 1, we indeed saw a clear cross-activation of relBEF in response to all toxins tested except YafQ. Induction of RelE, MazF, MqsR, HicA and HipA conferred a clear increase in the relBEF mRNA level in an hour. Use of three separate probes revealed, however, that different mRNA species pile up in response to different toxins. Before induction and 15 min after, all three probes – relB, relE and relF – detected a transcript of the same size corresponding to the full-length mRNA of the operon [45], as confirmed later by primer extension mapping of the 5′ end (Additional file 1: Figure S4). Only after MazF expression a shorter transcript, a putative cleavage product, could be detected at the 15 min time point using relE probe (Figure 1B). At later time points, hybridization with relB (Figure 1A) and relE (Figure 1B) probes gave different signals: in response to induction of MazF, MqsR, and HicA we saw cleavage of the full-length mRNA and massive accumulation of the toxin-encoding part, while the antitoxin-coding portion could not be detected and was apparently degraded (Figure 1A,B). Such cleavage and accumulation of the toxin portion also occurred in response to RelE. Hybridization with relF probe revealed additional cleavage, both within relE and downstream, in response to expression of all these toxins, and the relF part accumulated as the most abundant portion of the relBEF transcript (Figure 1C). Also, some transcripts larger than the full relBEF mRNA appeared, particularly after induction of RelE and MqsR. Production of HipA, which is not a ribonuclease, conferred strong induction of full-length relBEF mRNA but cleavage and uneven accumulation of different mRNA fragments could not be seen. MUP treatment produced overproduction of the full relBEF mRNA as well as accumulation of some cleavage products. Production of YafQ did not lead to a clear cross-activation of relBEF transcription. However, relE probe showed accumulation of a short RNA fragment in response to this toxin. It is possible, that transcription of the operon is activated by YafQ but the transcript is degraded to small fragments. Clearly, these fragments cannot serve as templates for synthesis of RelE and, therefore, functional cross-activation does not occur. Modest induction of relBEF with no cleavage was evident in the 1h and 2h samples of control cultures, lacking artificial production of any free toxin. We have to consider that, at this stage, the control cultures were approaching stationary phase, and induction of toxin-antitoxin modules has been described in similar conditions [48].

Probes complementary to yiaF and rpsS were used for control because the levels of transcription of these genes did not differ between log phase cells and the ampicillin-refractory non-growing subpopulation, where TA operons were highly expressed [38]. rpsS is a part of the large S10 ribosomal protein operon with an estimated transcribed length of 5181 bp [49]; yiaF (711 bp ORF) encodes for a putative membrane protein of unknown function; it is located between genes pointing in the opposite direction and must form a single-gene operon. The control mRNAs were not induced by toxins (Additional file 1: Figure S2B,C). After induction of toxins, the yiaF transcript was degraded without accumulation of any stable fragments. (Additional file 1: Figure S2B). Surprisingly, mupirocin initially induced transcription of yiaF whereas the level of the transcript dropped after longer incubation (Additional file 1: Figure S2B). The S10 transcript was degraded as well. Some accumulating stable fragments of the S10 transcript were detectable after MazF, RelE and MqsR production (Additional file 1: Figure S2C).

To be sure that the accumulating RNA fragments, which correspond to the 3′ portion of the relBEF mRNA, are not initiated from toxin-inducible cryptic promoters within the operon, we deleted the promoter of the relBEF operon. In the promoterless BW25113 ΔP relBEF strain, we did not see induction of the relBEF mRNA nor the characteristic accumulation of its 3′ portion (Additional file 1: Figure S3). We still saw a transcript that could be detected by the relE and relF probes (Additional file 1: Figure S3B,C) but the level of this transcript did not depend on the RelE production. It might be initiated from a constitutive promoter that was newly created by deletion of P relBEF . Transiently induced smear of RNA that was detected in BW25113 ΔP relBEF with the relB probe (Additional file 1: Figure S3A, lanes 6 and 7) is transcribed from the RelB-expression plasmid pKP3033. That is the reason why we omitted this plasmid when we studied induction of relBEF in response to RelE (Figure 1, Additional file 1: Figure S3, lanes 8–11). Thus, we can be sure that the shorter transcripts that massively pile up in response to toxins are indeed cleavage products and are initiated at the genuine P relBEF promoter.

Next, we tested whether over-production of the toxin RelE activates other toxin-antitoxin genes in the chromosome. The northern hybridization results show strong induction of the mqsRA, mazEF, dinJ-yafQ, hicAB, yefM-yoeB, and prlF-yhaV TA systems (Figure 2). Similarly to relBEF, the induced transcripts were cleaved and the toxin-encoding parts seem to accumulate preferentially while the antitoxin-coding parts are more effectively degraded. That appears to be true irrespective of whether the toxin is encoded by the first (mqsRA, hicAB) or the second (mazEF, yefM-yoeB, prlF-yhaV) gene of the operon (Figure 2). Reliable testing of this phenomenon requires characterization of the cleavage products and additional experiments in the future.

Additional experiments indicated that transcriptional cross-activation of TA operons does not occur between all possible TA combinations. Northern hybridization using mqsR probe showed that overproduction of MazF and HicA does not induce the mqsRA promoter while YafQ and HipA induce it (data not shown), as well as RelE (Figure 2).

Activation of mazEF by amino acid starvation is dependent on relBE

We wanted to test whether TA cross-activation happens also during natural physiological stresses. Amino acid starvation has been shown to induce transcription of the relBE[14] and mazEF[17] genes. We induced amino-acid starvation by addition of mupirocin to the cultures of BW25113 (wild type) and BW25113ΔrelBEF. Northern analysis indicated that transcription of mazEF is upregulated only in wild type bacteria and not in the relBE deficient strain (Figure 3B). Transcription of mqsRA, the other TA operon that we tested, was induced in both strains, independently of the RelBE system (Figure 3A). Thus, RelBE system activates another TA system, MazEF, in response to amino acid shortage. This evidences that TA cross-activation is not a mere artifact of toxin overexpression but occurs as a part of a real physiological response.
Figure 3
Figure 3

Transcription of mqsRA and mazEF operons in response to amino acid starvation. Mupirocin (MUP) was added to cultures of BW25113 (wt) and BW25113 ∆relBEF to inhibit isoleucine tRNA synthetase and induce stringent response. RNA was extracted at timepoints −1 (before addition of MUP), 15, 60, and 120 min; 10-μg aliquots were subjected to northern blotting and hybridized with probes mqsR (A) and mazF (B). The full-length mqsRA and mazEF transcripts are marked by arrowheads (◄). A longer mqsRA transcript can be seen above the marked band and has been described previously [59].

Cross-activation occurs in lon, ppk, clpP, and hslV deficient strains

Since it is widely accepted that TA loci are activated by proteolytic degradation of antitoxins, we tested whether transcriptional cross-activation is affected by Lon, ClpP or HslV proteases. Besides, we tested the requirement of polyphospate, which has been shown to activate Lon [50]. We expressed RelE, MazF, and MqsR toxins in BW25113 strain lacking lon or ppk, which encode for Lon and polyphosphate kinase, respectively, and observed chromosomal relBEF transcript by northern hybridization using probes relE and relF (Figure 4). Deletion of lon or ppk did not abolish cross-induction of relBEF by MqsR, and as seen on relF probed blot (Figure 4B), by MazF. We further tested relBEF activation in a double-knockout strain lacking Lon and ClpP, and a triple-knockout lacking Lon, ClpP and HslV proteases. Again, expression of MazF and MqsR obviously induced relBEF in the strains deficient for multiple proteases (Figure 4). Accumulating RelE-, MazF- and MqsR- specific cleavage intermediates produced similar patterns in all tested strains (Figure 1B,C, Figure 4). Production of YafQ did not cause a clear activation of relBEF transcription in the protease-deficient strains, similarly to the wt strain. Accumulation of a small fragment hybridizing to the relE probe can be detected in the ΔclpPX Δlon ΔhslVU strain (Figure 1B, Figure 4A). Ectopic production of RelE induced transcription of chromosomal relBEF in all strain backgrounds, as expected. Essentially, we can conclude that cross-activation of TA transcription occurs also in lon - , ppk - , clpPX - lon - , and clpPX - lon - hslVU - backgrounds.
Figure 4
Figure 4

Transcriptional activation of relBEF in protease- and polyphosphate kinase deficient strains. Cultures of BW25113 ∆lon, BW25113 ∆ppk, BW25113 ∆clpPX∆lon, and BW25113 ∆clpPX∆lon∆hslVU contained pVK11 (RelE), pSC3326 (MazF), pTX3 (MqsR), or pBAD-yafQ plasmid for toxin expression. Toxins were induced and RNA was extracted at timepoints −1 (before induction), 15 and 60 min; 10-μg aliquots were subjected to northern blotting and hybridized with probes relE (A) and relF (B). The full-length relBEF transcript is marked by arrowhead (◄).

Cleavage of the relBEF mRNA in vivo

To characterize the in vivo cleavage of relBEF mRNA in more detail, we mapped the 5′ ends of the cleavage products using primer extension analysis (Figure 5, Additional file 1: Figure S4, Table S3). As seen in Figure 5, the cleavage sites in the mRNA, which was purified from the cells with over-expression of the nucleases MqsR and HicA, are distributed all over the operon. Several specific cutting sites of the MazF nuclease are found in the RelB-encoding part. No cleavage is detected in response to production of the protein kinase HipA, as expected. Most of the cutting sites were unique for each toxin indicating that the cleavage in vivo was a result of primary activity of the over-produced toxin. RNA from MazF and MqsR over-expression samples was mostly cleaved at the specific cutting sites of these toxins, i.e. ACA [51] and GCU [16]. However, several unique cleavage sites in the MazF and MqsR over-expression samples do not contain these sequences and might be generated by unidentified ribonuclease(s), possibly cross-activated toxins (Additional file 1: Table S3). We also observed that not all ACA and GCU sequences were cleaved in the relBEF mRNA by MazF and MqsR, respectively. As before [19], the cleavage preferences of HicA could not be identified.
Figure 5
Figure 5

Cleavage of the relBEF mRNA in vivo . The same RNA samples that were analyzed by northern blotting (Figure 1) were subjected to primer extension analysis shown in (Additional file 1: Figure S4). Detected 5′ ends, localization of the extension primers and hybridization probes are mapped on to the relBEF operon. Dotted lines mark cleavage sites that occur in response to several over-produced toxins. The gray bar indicates the region where detection of the cleavage sites in the relBEF mRNA was impossible owing to the plasmidal relE mRNA transcribed from pVK11.

To confirm our notion of TA cross-activation, we hoped to see some cleavage hotspots. At those sites, strong cleavage by an overproduced toxin occurs at its specific cutting sequence (e.g. ACA in the case of MazF). Cleavage at the same site in response to expression of another toxin would indicate activation of the primary cutter by the over-produced toxin. We tested possible cross-activation at three of these sites. At position 174 (ˇACA), the relBEF transcript is cut by MazF and in response to the over-produced HicA. The MqsR-specific cleavage sites at positions 399 (GCˇU) and 431 (GˇCU) are also cleaved in the samples from HicA over-production (Additional file 1: Figure S4). We found that these cuts were not due to the activation of MazF and MqsR, since they occurred in RNA extracted from the BW25113ΔmazEF and BW25113ΔmqsRA cells (data not shown). ChpBK, a homolog of MazF with similar but relaxed sequence specificity [52] may be accountable for the cleavage at 174 (ˇACA).

The cleavage products of relBEF mRNA can be translated into proteins

The toxin-encoding parts of the TA transcripts seem to be generally more stable than the antitoxin-encoding parts and accumulate after cleavage (Figures 1, 2). If the toxin open reading frame (ORF) on these cleavage products is intact and translated into a functional protein, the T:A balance must be shifted towards toxin followed by more cleavage, cross-activation of other TA systems, and inhibition of protein synthesis. That creates the possibility of a positive feedback circuit and even a network of them. A positive autoregulatory loop, in turn, could explain the bistability of bacterial growth observed in response to toxin expression [53, 54].

To test whether proteins are translated from the cleaved relBEF mRNA, we used the T7 promoter for expression of two transcripts, which begin at the sites of MazF-inflicted cleavage, at positions +28 and +148 from the 5′ end of the full-length transcript, and extend downstream of the relE ORF. The +28 RNA starts immediately upstream of the relB ORF (Additional file 1: Figure S4). Thus, the relB ORF is leaderless and lacks the upstream untranslated region with the ribosome binding site (RBS). The +148 RNA starts in the middle of the relB ORF. To allow RelE to be detected, we added the His6 tag to the C-terminus of the toxin and introduced substitutions R81A and R83A, which reduce its toxicity [55]. Expression of these RNAs in BL21(DE3) resulted in production of the toxin RelE(R81A/R83A)-C-His, although in smaller quantities than from the control transcript with the intact 5′ end (Figure 6). Thus, the accumulating cleavage products of TA mRNA can be translated into proteins, although less effectively than full transcripts with intact RBS in front of relB. Reduced translation of the downstream relE(R81A/R83A)-C-His open reading frame in shorter transcripts suggests that relE lacks its own RBS and it is produced due to translational coupling of relBE genes. Translational coupling of polycistronic TA mRNA has been demonstrated previously for parD (kis-kid) of plasmid R1 [56].
Figure 6
Figure 6

RelE toxin can be translated from mRNAs resembling the accumulating cleavage fragments of the relBEF transcript. Cultures of BL21(DE3) contained plasmid pNK31 for T7 expression of an mRNA starting at the 5′end of the full-length (FL) relBEF transcript; pNK32 for expression of an mRNA starting at the position + 28; and pNK33 for expression of an mRNA with disrupted relB open reading frame starting at position +148. Expression of T7 RNA polymerase was induced for 1 h by adding 1mM IPTG. Control cultures were grown without IPTG. Total protein lysates were analyzed for expression of RelE(R81A/R83A)-C-His using western blotting (A), and RNA expression was analyzed by northern hybridization using oligoprobe relE (B).

Transient expression of toxins can induce bistability of growth

Production of toxins causes an extensive rearrangement of bacterial physiology. It can inflict dormancy and antibiotic tolerance [57] if the toxin level exceeds a threshold [54]. Fluctuations in toxin levels above and below the threshold have been used to explain the coexistence of dormant and growing cells in a population [54]. The possibility of positive feedback by the generation and selective buildup of the toxin-encoding mRNA fragments may explain this heterogeneity in growth. Therefore, we wanted to evaluate the recovery of single bacteria and test possible growth heterogeneity after over-production of a toxin and the resulting activation of the chromosomal TA loci. We monitored growth resumption by individual cells using dilution of previously synthesized green fluorescent protein (GFP) [58]. The plasmid pTM11 was inserted into the chromosome of BW25311 to allow IPTG-inducible GFP to be expressed, and this strain was transformed with plasmids for L-arabinose-inducible production of toxins RelE, MazF, MqsR and HipA. Expression of GFP was induced for 2.5 h; thereafter, the cells were transferred into medium containing L-arabinose to induce the toxins. After 90 min, the growth medium was changed again to shut down toxin synthesis and allow recovery (Additional file 1: Figure S5). Analysis of the bacterial GFP content by flow cytometry (Additional file 1: Figure S6) showed that after temporary expression of RelE and HipA the bacteria resumed growth rather uniformly, while after expression of MazF and MqsR a subpopulation started to grow with a delay. Thus, expression of these toxins created bistability in a population. Most importantly, all bacteria resumed growth after the transient expression of toxins. Although inhibition by MazF and MqsR was apparently stronger and induced growth heterogeneity, it did not generate a subpopulation of persistently non-dividing bacteria (Additional file 1: Figure S6).

Discussion

Mutual cross-activation of TA systems

Sequential or simultaneous activation of different TA systems has been reported elsewhere. Transcription of several TA operons was induced in the persister-enriched subpopulation [38, 39]. Amino acid starvation in E. coli activated both RelE and MazF (ChpAK) [14, 17]. We observed induction of the mqsRA system in response to HipA activation [59], whereas overproduction of MqsR induced transcription of relBE and relF(hokD) [60]. Also, ectopic expression of VapC toxins originating from Salmonella and Shigella activated YoeB [61] and production of the Doc toxin activated RelE in E. coli[62]. Here, we show that overexpression of several toxins can activate transcription of the other TA operons. Since toxins and TA operons in this study present a random sample, such cross-interactions might be common and be the rule rather than the exception. Consequently, TA systems have a potential to form a cross-activation network, which operates at the transcriptional level (Figure 7). The presence of such network versus lone and uncoordinated TA systems must have an impact on TA activity during the stress response and setup of dormancy.
Figure 7
Figure 7

Toxin-antitoxin systems are subject to both auto- and cross-regulation. Cognate regulatory interactions are in red and non-cognate interactions are in blue. According to the established model, cognate antitoxin and toxin, which are encoded by co-transcribed genes, form a tight complex and antitoxin inhibits the toxin through direct protein-protein interaction. Antitoxin, both alone and in complex with the toxin, binds to the operator DNA and auto-represses transcription of the TA operon. Free toxin in excess disrupts this DNA-protein interaction and induces transcriptional de-repression. We show that transcription of TA genes can be induced also by non-cognate toxins. Moreover, cleavage of the TA mRNA by both cognate and non-cognate toxins results in accumulation of the toxin-encoding mRNA fragments. Translation of these fragments can lead to accumulation of free toxin.

Induction of the chromosomal relBEF in response to the ectopically produced RelE can be explained by conditional cooperativity (dependence of transcriptional regulation on the T:A ratio) [35]. However, according to our current knowledge, such mechanism is not applicable to cross-induction. Activation of YoeB by VapC depended on Lon protease [61]. Also, Lon was required for induction of TA operons in response to amino acid starvation and chloramphenicol [14, 17, 18, 61]. Our experiments do not provide a solid support for the role of Lon and ClpP in cross-regulation between TA systems of E. coli (Figure 4). Since the cross-induction was present in the knock-out strains, an additional, Lon-, ClpP-, HslV-, and polyphosphate-independent mechanism of regulation must be involved. Unlocking this mechanism remains a task for future studies. The simplest explanation to activation of TA systems would be depletion of antitoxins. It must inevitably happen when protein synthesis decreases. That predicts nonselective induction of all TA operons in response to inhibition of translation, no matter if it is caused by starvation or artificial production of a toxin. Requirement of relBE for transcriptional activation of mazEF during amino acid starvation (Figure 3) contradicts this prediction as well as the lack of mqsRA induction in response to overproduction of MazF and HicA (data not shown). An option for a mechanism of cross-activation is positive feedback regulation due to selective accumulation of toxin-encoding fragments upon mRNA cleavage. As we saw, after cleavage by overproduced toxin, the antitoxin-encoding RNA fragments are rapidly degraded while the toxin-encoding fragments may serve as templates for translation of toxin. Different toxins produce different cleavage products. That can potentially explain why they cause unequal level of trans-activation when overproduced.

Another intriguing issue of TA cross-reaction is the possible cross-inhibition due to non-cognate interactions. Some authors report such cross-reactions [63–68] while others have tested but not found them [69, 70]. As a part of this study, we examined non-cognate inhibition between E. coli toxins and antitoxins of the RelBE, MazEF, MqsRA, and HipBA systems in vivo. In this attempt, we run into a previously described phenomenon that may become a source of erroneous results. If toxins are expressed from the arabinose-inducible PBAD promoter and antitoxins from an IPTG-inducible promoter, it is important to consider that IPTG inhibits PBAD directly [71]. When we used an expression vector that encoded for the IPTG-insensitive C280* version of AraC transcriptional activator, we could not see any cross-inhibition. Based on that, a recent report on functional non-cognate TA interactions in Mycobacterium tuberculosis[67] may require retesting.

Selective targeting of mRNA by toxins as a mechanism of gene regulation

In the current study, we found that the cleavage products produced by TA toxins differ in stability. Selective targeting of mRNAs by endoribonucleolytic toxins and different stabilities of the resulting cleavage products may constitute another layer of gene regulation in the bacterial stress response. Differences in half-life and translational efficiency of mRNA cleavage products, along with generation of a pool of ribosomes lacking the anti-Shine-Dalgarno sequence (as shown for MazF [22]), could profoundly affect the proteome composition. An example of such an effect is the occurrence of a MazF-resistant protein pool in E. coli[72]. The accumulation of toxin-encoding mRNA fragments may have potential use as a marker of toxin activation in studies of stressed and non-growing bacteria. Increase of the T/A ratio may possibly trigger a positive feedback loop consisting of transcriptional activation of the TA operon, successive cleavage of the TA transcript, buildup of the toxin-encoding mRNA fragments, and translation of them, shifting the T/A balance (Figure 7). Thus, it can be related to TA-linked growth heterogeneity in bacterial populations (Additional file 1: Figure S6) [38, 39, 54].

Conclusions

The main finding of this study is that bacterial toxin-antitoxin systems affect mutually each others’ expression and activity (Figure 7). We show that overexpression of one toxin can activate transcription of the other TA operons. Toxins with endoribonuclease activity add another layer of complexity to these interactions. They cleave TA mRNA, which is followed by degradation of the antitoxin-encoding RNA fragments and accumulation of the toxin-encoding fragments. We show that these accumulating mRNA fragments can be translated to produce more toxin.

Most of bacteria have many different TA systems. Although their function is debatable, many TA toxins have similar activity and the inhibitory effect on bacterial cells is common to all of them. Therefore, an important question is whether TA systems are redundant or not. Another intriguing issue is whether different TA systems are functionally connected and do cross-talk [44, 70].

Here we over-expressed toxins to show that TA systems have a potential to form a network of cross-reacting regulators in E. coli. We found an example of such cross-reaction, which occurs without artificial overexpression: the relBE-dependent transcriptional activation of mazEF during amino acid starvation. It remains a rather difficult task to identify the mechanism(s) of TA cross-activation. Currently we know that cross-activation is not dependent on major proteases Lon, ClpP, and HslV. Also, it cannot be a self-evident outcome of antitoxin shortage since we know examples where shutdown of protein synthesis does not activate a TA promoter.

Methods

Bacterial strains, plasmids and growth conditions

All strains and plasmids are listed in Additional file 1: Table S1. Conditions of bacterial cultivation and construction of strains and plasmids are described in Additional file 1: Supporting information.

Northern hybridization

Procedures for blotting and hybridization are described in [59]. E. coli BW25113 was transformed with two plasmids, one bearing an antitoxin gene and the other bearing a toxin gene. Cultures containing the empty vector plasmids pBAD33 and pOU82 were used for negative controls. When bacteria contained plasmids for toxin expression, the LB medium for overnight cultures was supplemented with 0.2% glucose and 50 μM IPTG (for HicA with 1mM L-arabinose). Overnight cultures were diluted 1000-fold into 200 ml of LB and grown to OD600 ≈ 0.2 (for ~ 2.5 h). To induce toxins, 1 mM L-arabinose, 1 mM IPTG (for HicA) or 30 μg ml−1 mupirocin was added. Overnight cultures of BW25113 ΔrelBEF and BW25113 ΔP relBEF containing plasmids were diluted into LB supplemented with 0.2% glucose and 50 μM IPTG; at OD600 ≈ 0.2, bacteria were collected by centrifugation (5 min, 5000g, at 20°C) and resuspended in prewarmed LB supplemented with 1 mM L-arabinose. Total RNA was extracted using two different protocols: in Figures 2, 6 and S3 we used Trizol reagent [59] and in all other experiments we used hot phenol (for details see Additional file 1: Supporting information). Samples of total RNA (10 μg) were subjected to electrophoresis on denaturing gels. The DNA oligoprobes used for hybridization are listed in Table S2 (Additional file 1). For re-hybridization, the membranes were stripped by boiling for 2×10 min in 0.1% SDS, 5mM EDTA. Chemiluminescent signals were captured using ImageQuant RT ECL imager (GE Healthcare) and X-ray film (Agfa).

Primer extension

RNA samples were collected as for northern blotting. Extension primers (Additional file 1: Table S2) were labeled with [γ32P]ATP by T4 polynucleotide kinase (Thermo Scientific) and purified with a Nucleotide Removal Kit (Qiagen). Total RNA (15 μg) was mixed with labeled primer and incubated at 75°C for 2 min followed by slow cooling for 25 min. Extension reactions were carried out at 44°C for 30 min using 200U of RevertAidTM H minus reverse transcriptase (Thermo Scientific) and stopped with 10 μl of formamide loading buffer [73]. Reaction products were concentrated by ethanol precipitation before gel electrophoresis. DNA was sequenced using a Sequenase Version 2.0 Kit (USB Products, Affymetrics). A PCR product amplified using primers relBEFup and relFdwn, and treated with Exonuclease I and shrimp alkaline phosphatase (ThermoScientific), was used as the template for the sequencing reactions. Samples were analyzed by 7M urea-6% polyacrylamide gel electrophoresis.

Protein electrophoresis and western blots

To prepare lysates, bacteria were grown to an OD600 of ~0.7 and expression of T7 RNA polymerase was induced for 1 h by adding 1mM IPTG. Control cultures were grown without IPTG. Bacteria were spinned down and lysed in Laemmli sample buffer. Proteins were separated by tricin–SDS–13% polyacrylamide gel electrophoresis [74]. For detection of the His6-tagged toxins, the proteins were electroblotted onto Hybond-ECL nitrocellulose membrane filters (GE Healthcare) and probed with nickel-activated horseradish peroxidase (HisProbeTM-HRP; Thermo Scientific).

Growth resumption experiments

Overnight cultures were grown from fresh single colonies for 17–18 h in LB supplemented with 0.2% glucose and diluted 500-fold, into 3 ml of broth. After 2 h of incubation, 1 mM IPTG was added to initiate synthesis of green fluorescent protein (GFP). Expression of GFP was induced for 2.5 h. Then, cells were collected by centrifugation and transferred into LB supplemented with 0.2% L-arabinose to induce toxin synthesis. During the change of the medium, the culture was diluted 10-fold. After 90 min, the growth medium was changed to LB containing 0.2% glucose to stop the production of toxins, this time with 2-fold dilution. Starting from the induction of toxin synthesis, samples were taken for flow cytometry analysis and OD600 measurement. For flow cytometry analysis, the samples were mixed with an equal volume of 30% glycerol in PBS and stored at −80°C pending analysis. After dilution with sterile PBS, the samples were analyzed using an LSRII and a high-throughput sampler (BD) with a laser beam maximum wavelength of 488 nm. The results were analyzed by using FlowJo 7.2.1software.

Reproducibility of experiments

All growth inhibition (Additional file 1: Figure S1) and growth resumption experiments (Additional file 1: Figure S5, S6) were repeated at least three times. All northern blot (Figures 1, 2, 3, 4, 6 Additional file 1: Figures S2, S3), primer extension mapping (Additional file 1: Figure S4) and in vivo translation experiments (Figure 6) were repeated at least twice with similar results. Typical results are presented for these experiments and for the FACS analysis of growth resumption (Additional file 1: Figure S6).

Declarations

Acknowledgements

This work was supported by Estonian Science Foundation grant 8822 and by the European Regional Development Fund through the Center of Excellence in Chemical Biology. We thank Kenn Gerdes, Edita Sužiedėlienė, and Kim Lewis for plasmids and strains; and Vasili Hauryliuk, Ülo Maiväli, Isabella Moll and Arvi Jõers for comments on the manuscript. The authors would like to thank the anonymous reviewer who suggested the mupirocin experiment as a test for the TA cross-activation in physiologically relevant conditions.

Authors’ Affiliations

(1)
Institute of Technology, University of Tartu, Nooruse 1, 50411 Tartu, Estonia

References

  1. Yamaguchi Y, Inouye M: Regulation of growth and death in Escherichia coli by toxin-antitoxin systems. Nat Rev Microbiol. 2011, 9 (11): 779-790. 10.1038/nrmicro2651.PubMedView ArticleGoogle Scholar
  2. Yamaguchi Y, Park JH, Inouye M: Toxin-antitoxin systems in bacteria and archaea. Annu Rev Genet. 2011, 45: 61-79. 10.1146/annurev-genet-110410-132412.PubMedView ArticleGoogle Scholar
  3. Shao Y, Harrison EM, Bi D, Tai C, He X, Ou HY, Rajakumar K, Deng Z: TADB: a web-based resource for type 2 toxin-antitoxin loci in bacteria and archaea. Nucleic Acids Res. 2011, 39 (Database issue): D606-611.PubMedPubMed CentralView ArticleGoogle Scholar
  4. Pandey DP, Gerdes K: Toxin-antitoxin loci are highly abundant in free-living but lost from host-associated prokaryotes. Nucleic Acids Res. 2005, 33 (3): 966-976. 10.1093/nar/gki201.PubMedPubMed CentralView ArticleGoogle Scholar
  5. Makarova KS, Wolf YI, Koonin EV: Comprehensive comparative-genomic analysis of type 2 toxin-antitoxin systems and related mobile stress response systems in prokaryotes. Biol Direct. 2009, 4: 19-10.1186/1745-6150-4-19.PubMedPubMed CentralView ArticleGoogle Scholar
  6. Leplae R, Geeraerts D, Hallez R, Guglielmini J, Dreze P, Van Melderen L: Diversity of bacterial type II toxin-antitoxin systems: a comprehensive search and functional analysis of novel families. Nucleic Acids Res. 2011, 39 (13): 5513-5525. 10.1093/nar/gkr131.PubMedPubMed CentralView ArticleGoogle Scholar
  7. Magnuson RD: Hypothetical functions of toxin-antitoxin systems. J Bacteriol. 2007, 189 (17): 6089-6092. 10.1128/JB.00958-07.PubMedPubMed CentralView ArticleGoogle Scholar
  8. Van Melderen L, Saavedra De Bast M: Bacterial toxin-antitoxin systems: more than selfish entities?. PLoS Genet. 2009, 5 (3): e1000437-10.1371/journal.pgen.1000437.PubMedPubMed CentralView ArticleGoogle Scholar
  9. Tsilibaris V, Maenhaut-Michel G, Mine N, Van Melderen L: What is the benefit to Escherichia coli of having multiple toxin-antitoxin systems in its genome?. J Bacteriol. 2007, 189 (17): 6101-6108. 10.1128/JB.00527-07.PubMedPubMed CentralView ArticleGoogle Scholar
  10. Yarmolinsky MB: Programmed cell death in bacterial populations. Science. 1995, 267 (5199): 836-837. 10.1126/science.7846528.PubMedView ArticleGoogle Scholar
  11. Sayeed S, Brendler T, Davis M, Reaves L, Austin S: Surprising dependence on postsegregational killing of host cells for maintenance of the large virulence plasmid of Shigella flexneri. J Bacteriol. 2005, 187 (8): 2768-2773. 10.1128/JB.187.8.2768-2773.2005.PubMedPubMed CentralView ArticleGoogle Scholar
  12. Masuda Y, Miyakawa K, Nishimura Y, Ohtsubo E: chpA and chpB, Escherichia coli chromosomal homologs of the pem locus responsible for stable maintenance of plasmid R100. J Bacteriol. 1993, 175 (21): 6850-6856.PubMedPubMed CentralGoogle Scholar
  13. Gotfredsen M, Gerdes K: The Escherichia coli relBE genes belong to a new toxin-antitoxin gene family. Mol Microbiol. 1998, 29 (4): 1065-1076. 10.1046/j.1365-2958.1998.00993.x.PubMedView ArticleGoogle Scholar
  14. Christensen SK, Mikkelsen M, Pedersen K, Gerdes K: RelE, a global inhibitor of translation, is activated during nutritional stress. Proc Natl Acad Sci USA. 2001, 98 (25): 14328-14333. 10.1073/pnas.251327898.PubMedPubMed CentralView ArticleGoogle Scholar
  15. Aizenman E, Engelberg-Kulka H, Glaser G: An Escherichia coli chromosomal “addiction module” regulated by guanosine [corrected] 3′,5′-bispyrophosphate: a model for programmed bacterial cell death. Proc Natl Acad Sci USA. 1996, 93 (12): 6059-6063. 10.1073/pnas.93.12.6059.PubMedPubMed CentralView ArticleGoogle Scholar
  16. Yamaguchi Y, Park JH, Inouye M: MqsR, a crucial regulator for quorum sensing and biofilm formation, is a GCU-specific mRNA interferase in Escherichia coli. J Biol Chem. 2009, 284 (42): 28746-28753. 10.1074/jbc.M109.032904.PubMedPubMed CentralView ArticleGoogle Scholar
  17. Christensen SK, Pedersen K, Hansen FG, Gerdes K: Toxin-antitoxin loci as stress-response-elements: ChpAK/MazF and ChpBK cleave translated RNAs and are counteracted by tmRNA. J Mol Biol. 2003, 332 (4): 809-819. 10.1016/S0022-2836(03)00922-7.PubMedView ArticleGoogle Scholar
  18. Christensen-Dalsgaard M, Gerdes K: Two higBA loci in the Vibrio cholerae superintegron encode mRNA cleaving enzymes and can stabilize plasmids. Mol Microbiol. 2006, 62 (2): 397-411. 10.1111/j.1365-2958.2006.05385.x.PubMedView ArticleGoogle Scholar
  19. Jorgensen MG, Pandey DP, Jaskolska M, Gerdes K: HicA of Escherichia coli defines a novel family of translation-independent mRNA interferases in bacteria and archaea. J Bacteriol. 2009, 191 (4): 1191-1199. 10.1128/JB.01013-08.PubMedPubMed CentralView ArticleGoogle Scholar
  20. Pedersen K, Zavialov AV, Pavlov MY, Elf J, Gerdes K, Ehrenberg M: The bacterial toxin RelE displays codon-specific cleavage of mRNAs in the ribosomal a site. Cell. 2003, 112 (1): 131-140. 10.1016/S0092-8674(02)01248-5.PubMedView ArticleGoogle Scholar
  21. Prysak MH, Mozdzierz CJ, Cook AM, Zhu L, Zhang Y, Inouye M, Woychik NA: Bacterial toxin YafQ is an endoribonuclease that associates with the ribosome and blocks translation elongation through sequence-specific and frame-dependent mRNA cleavage. Mol Microbiol. 2009, 71 (5): 1071-1087. 10.1111/j.1365-2958.2008.06572.x.PubMedView ArticleGoogle Scholar
  22. 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 (1): 147-157. 10.1016/j.cell.2011.07.047.PubMedView ArticleGoogle Scholar
  23. Winther KS, Gerdes K: Enteric virulence associated protein VapC inhibits translation by cleavage of initiator tRNA. Proc Natl Acad Sci USA. 2011, 108 (18): 7403-7407. 10.1073/pnas.1019587108.PubMedPubMed CentralView ArticleGoogle Scholar
  24. Bernard P, Couturier M: Cell killing by the F plasmid CcdB protein involves poisoning of DNA-topoisomerase II complexes. J Mol Biol. 1992, 226 (3): 735-745. 10.1016/0022-2836(92)90629-X.PubMedView ArticleGoogle Scholar
  25. Jiang Y, Pogliano J, Helinski DR, Konieczny I: ParE toxin encoded by the broad-host-range plasmid RK2 is an inhibitor of Escherichia coli gyrase. Mol Microbiol. 2002, 44 (4): 971-979. 10.1046/j.1365-2958.2002.02921.x.PubMedView ArticleGoogle Scholar
  26. Schumacher MA, Piro KM, Xu W, Hansen S, Lewis K, Brennan RG: Molecular mechanisms of HipA-mediated multidrug tolerance and its neutralization by HipB. Science. 2009, 323 (5912): 396-401. 10.1126/science.1163806.PubMedPubMed CentralView ArticleGoogle Scholar
  27. Correia FF, D’Onofrio A, Rejtar T, Li L, Karger BL, Makarova K, Koonin EV, Lewis K: Kinase activity of overexpressed HipA is required for growth arrest and multidrug tolerance in Escherichia coli. J Bacteriol. 2006, 188 (24): 8360-8367. 10.1128/JB.01237-06.PubMedPubMed CentralView ArticleGoogle Scholar
  28. Mutschler H, Gebhardt M, Shoeman RL, Meinhart A: A novel mechanism of programmed cell death in bacteria by toxin-antitoxin systems corrupts peptidoglycan synthesis. PLoS Biol. 2011, 9 (3): e1001033-10.1371/journal.pbio.1001033.PubMedPubMed CentralView ArticleGoogle Scholar
  29. Pedersen K, Christensen SK, Gerdes K: Rapid induction and reversal of a bacteriostatic condition by controlled expression of toxins and antitoxins. Mol Microbiol. 2002, 45 (2): 501-510. 10.1046/j.1365-2958.2002.03027.x.PubMedView ArticleGoogle Scholar
  30. Amitai S, Yassin Y, Engelberg-Kulka H: MazF-mediated cell death in Escherichia coli: a point of no return. J Bacteriol. 2004, 186 (24): 8295-8300. 10.1128/JB.186.24.8295-8300.2004.PubMedPubMed CentralView ArticleGoogle Scholar
  31. Hazan R, Sat B, Engelberg-Kulka H: Escherichia coli mazEF-mediated cell death is triggered by various stressful conditions. J Bacteriol. 2004, 186 (11): 3663-3669. 10.1128/JB.186.11.3663-3669.2004.PubMedPubMed CentralView ArticleGoogle Scholar
  32. Nariya H, Inouye M: MazF, an mRNA interferase, mediates programmed cell death during multicellular Myxococcus development. Cell. 2008, 132 (1): 55-66. 10.1016/j.cell.2007.11.044.PubMedView ArticleGoogle Scholar
  33. Gerdes K, Christensen SK, Lobner-Olesen A: Prokaryotic toxin-antitoxin stress response loci. Nat Rev Microbiol. 2005, 3 (5): 371-382. 10.1038/nrmicro1147.PubMedView ArticleGoogle Scholar
  34. Cataudella I, Trusina A, Sneppen K, Gerdes K, Mitarai N: Conditional cooperativity in toxin-antitoxin regulation prevents random toxin activation and promotes fast translational recovery. Nucleic Acids Res. 2012, 40 (14): 6424-6434. 10.1093/nar/gks297.PubMedPubMed CentralView ArticleGoogle Scholar
  35. Overgaard M, Borch J, Jorgensen MG, Gerdes K: Messenger RNA interferase RelE controls relBE transcription by conditional cooperativity. Mol Microbiol. 2008, 69 (4): 841-857. 10.1111/j.1365-2958.2008.06313.x.PubMedView ArticleGoogle Scholar
  36. Boggild A, Sofos N, Andersen KR, Feddersen A, Easter AD, Passmore LA, Brodersen DE: The crystal structure of the intact E. coli RelBE toxin-antitoxin complex provides the structural basis for conditional cooperativity. Structure. 2012, 20 (10): 1641-1648. 10.1016/j.str.2012.08.017.PubMedPubMed CentralView ArticleGoogle Scholar
  37. Winther KS, Gerdes K: Regulation of enteric vapBC transcription: induction by VapC toxin dimer-breaking. Nucleic Acids Res. 2012, 40 (10): 4347-4357. 10.1093/nar/gks029.PubMedPubMed CentralView ArticleGoogle Scholar
  38. Keren I, Shah D, Spoering A, Kaldalu N, Lewis K: Specialized persister cells and the mechanism of multidrug tolerance in Escherichia coli. J Bacteriol. 2004, 186 (24): 8172-8180. 10.1128/JB.186.24.8172-8180.2004.PubMedPubMed CentralView ArticleGoogle Scholar
  39. Shah D, Zhang Z, Khodursky A, Kaldalu N, Kurg K, Lewis K: Persisters: a distinct physiological state of E. coli. BMC Microbiol. 2006, 6: 53-10.1186/1471-2180-6-53.PubMedPubMed CentralView ArticleGoogle Scholar
  40. Lewis K: Persister cells. Annu Rev Microbiol. 2010, 64: 357-372. 10.1146/annurev.micro.112408.134306.PubMedView ArticleGoogle Scholar
  41. Hong SH, Wang X, O’Connor HF, Benedik MJ, Wood TK: Bacterial persistence increases as environmental fitness decreases. Microb Biotechnol. 2012, 5 (4): 509-522. 10.1111/j.1751-7915.2011.00327.x.PubMedPubMed CentralView ArticleGoogle Scholar
  42. Moyed HS, Bertrand KP: HipA, a newly recognized gene of Escherichia coli K-12 that affects frequency of persistence after inhibition of murein synthesis. J Bacteriol. 1983, 155 (2): 768-775.PubMedPubMed CentralGoogle Scholar
  43. Harrison JJ, Wade WD, Akierman S, Vacchi-Suzzi C, Stremick CA, Turner RJ, Ceri H: The chromosomal toxin gene yafQ is a determinant of multidrug tolerance for Escherichia coli growing in a biofilm. Antimicrob Agents Chemother. 2009, 53 (6): 2253-2258. 10.1128/AAC.00043-09.PubMedPubMed CentralView ArticleGoogle Scholar
  44. Maisonneuve E, Shakespeare LJ, Jorgensen MG, Gerdes K: Bacterial persistence by RNA endonucleases. Proc Natl Acad Sci USA. 2011, 108 (32): 13206-13211. 10.1073/pnas.1100186108.PubMedPubMed CentralView ArticleGoogle Scholar
  45. Bech FW, Jorgensen ST, Diderichsen B, Karlstrom OH: Sequence of the relB transcription unit from Escherichia coli and identification of the relB gene. EMBO J. 1985, 4 (4): 1059-1066.PubMedPubMed CentralGoogle Scholar
  46. Gerdes K, Bech FW, Jorgensen ST, Lobner-Olesen A, Rasmussen PB, Atlung T, Boe L, Karlstrom O, Molin S, von Meyenburg K: Mechanism of postsegregational killing by the hok gene product of the parB system of plasmid R1 and its homology with the relF gene product of the E. coli relB operon. EMBO J. 1986, 5 (8): 2023-2029.PubMedPubMed CentralGoogle Scholar
  47. Reiss S, Pane-Farre J, Fuchs S, Francois P, Liebeke M, Schrenzel J, Lindequist U, Lalk M, Wolz C, Hecker M: Global analysis of the Staphylococcus aureus response to mupirocin. Antimicrob Agents Chemother. 2012, 56 (2): 787-804. 10.1128/AAC.05363-11.PubMedPubMed CentralView ArticleGoogle Scholar
  48. Sangurdekar DP, Srienc F, Khodursky AB: A classification based framework for quantitative description of large-scale microarray data. Genome Biol. 2006, 7 (4): R32-10.1186/gb-2006-7-4-r32.PubMedPubMed CentralView ArticleGoogle Scholar
  49. Zurawski G, Zurawski SM: Structure of the Escherichia coli S10 ribosomal protein operon. Nucleic Acids Res. 1985, 13 (12): 4521-4526. 10.1093/nar/13.12.4521.PubMedPubMed CentralView ArticleGoogle Scholar
  50. Kuroda A, Nomura K, Ohtomo R, Kato J, Ikeda T, Takiguchi N, Ohtake H, Kornberg A: Role of inorganic polyphosphate in promoting ribosomal protein degradation by the Lon protease in E. coli. Science. 2001, 293 (5530): 705-708. 10.1126/science.1061315.PubMedView ArticleGoogle Scholar
  51. Zhang Y, Zhang J, Hara H, Kato I, Inouye M: Insights into the mRNA cleavage mechanism by MazF, an mRNA interferase. J Biol Chem. 2005, 280 (5): 3143-3150.PubMedView ArticleGoogle Scholar
  52. Zhang Y, Zhu L, Zhang J, Inouye M: Characterization of ChpBK, an mRNA interferase from Escherichia coli. J Biol Chem. 2005, 280 (28): 26080-26088. 10.1074/jbc.M502050200.PubMedView ArticleGoogle Scholar
  53. Dubnau D, Losick R: Bistability in bacteria. Mol Microbiol. 2006, 61 (3): 564-572. 10.1111/j.1365-2958.2006.05249.x.PubMedView ArticleGoogle Scholar
  54. Rotem E, Loinger A, Ronin I, Levin-Reisman I, Gabay C, Shoresh N, Biham O, Balaban NQ: Regulation of phenotypic variability by a threshold-based mechanism underlies bacterial persistence. Proc Natl Acad Sci USA. 2010, 107 (28): 12541-12546. 10.1073/pnas.1004333107.PubMedPubMed CentralView ArticleGoogle Scholar
  55. Li GY, Zhang Y, Inouye M, Ikura M: Inhibitory mechanism of Escherichia coli RelE-RelB toxin-antitoxin module involves a helix displacement near an mRNA interferase active site. J Biol Chem. 2009, 284 (21): 14628-14636. 10.1074/jbc.M809656200.PubMedPubMed CentralView ArticleGoogle Scholar
  56. Ruiz-Echevarria MJ, de la Cueva G, Diaz-Orejas R: Translational coupling and limited degradation of a polycistronic messenger modulate differential gene expression in the parD stability system of plasmid R1. Mol Gen Genet. 1995, 248 (5): 599-609. 10.1007/BF02423456.PubMedView ArticleGoogle Scholar
  57. Vazquez-Laslop N, Lee H, Neyfakh AA: Increased persistence in Escherichia coli caused by controlled expression of toxins or other unrelated proteins. J Bacteriol. 2006, 188 (10): 3494-3497. 10.1128/JB.188.10.3494-3497.2006.PubMedPubMed CentralView ArticleGoogle Scholar
  58. Roostalu J, Joers A, Luidalepp H, Kaldalu N, Tenson T: Cell division in Escherichia coli cultures monitored at single cell resolution. BMC Microbiol. 2008, 8: 68-10.1186/1471-2180-8-68.PubMedPubMed CentralView ArticleGoogle Scholar
  59. Kasari V, Kurg K, Margus T, Tenson T, Kaldalu N: The Escherichia coli mqsR and ygiT genes encode a new toxin-antitoxin pair. J Bacteriol. 2010, 192 (11): 2908-2919. 10.1128/JB.01266-09.PubMedPubMed CentralView ArticleGoogle Scholar
  60. Kim Y, Wang X, Zhang XS, Grigoriu S, Page R, Peti W, Wood TK: Escherichia coli toxin/antitoxin pair MqsR/MqsA regulate toxin CspD. Environ Microbiol. 2010, 12 (5): 1105-1121. 10.1111/j.1462-2920.2009.02147.x.PubMedPubMed CentralView ArticleGoogle Scholar
  61. Winther KS, Gerdes K: Ectopic production of VapCs from enterobacteria inhibits translation and trans-activates YoeB mRNA interferase. Mol Microbiol. 2009, 72 (4): 918-930. 10.1111/j.1365-2958.2009.06694.x.PubMedView ArticleGoogle Scholar
  62. Garcia-Pino A, Christensen-Dalsgaard M, Wyns L, Yarmolinsky M, Magnuson RD, Gerdes K, Loris R: Doc of prophage P1 is inhibited by its antitoxin partner Phd through fold complementation. J Biol Chem. 2008, 283 (45): 30821-30827. 10.1074/jbc.M805654200.PubMedPubMed CentralView ArticleGoogle Scholar
  63. Santos Sierra S, Giraldo R, Diaz Orejas R: Functional interactions between chpB and parD, two homologous conditional killer systems found in the Escherichia coli chromosome and in plasmid R1. FEMS Microbiol Lett. 1998, 168 (1): 51-58. 10.1111/j.1574-6968.1998.tb13254.x.PubMedView ArticleGoogle Scholar
  64. Santos-Sierra S, Giraldo R, Diaz-Orejas R: Functional interactions between homologous conditional killer systems of plasmid and chromosomal origin. FEMS Microbiol Lett. 1997, 152 (1): 51-56. 10.1111/j.1574-6968.1997.tb10408.x.PubMedView ArticleGoogle Scholar
  65. Wilbaux M, Mine N, Guerout AM, Mazel D, Van Melderen L: Functional interactions between coexisting toxin-antitoxin systems of the ccd family in Escherichia coli O157:H7. J Bacteriol. 2007, 189 (7): 2712-2719. 10.1128/JB.01679-06.PubMedPubMed CentralView ArticleGoogle Scholar
  66. Grady R, Hayes F: Axe-Txe, a broad-spectrum proteic toxin-antitoxin system specified by a multidrug-resistant, clinical isolate of enterococcus faecium. Mol Microbiol. 2003, 47 (5): 1419-1432. 10.1046/j.1365-2958.2003.03387.x.PubMedView ArticleGoogle Scholar
  67. Zhu L, Sharp JD, Kobayashi H, Woychik NA, Inouye M: Noncognate Mycobacterium tuberculosis toxin-antitoxins can physically and functionally interact. J Biol Chem. 2010, 285 (51): 39732-39738. 10.1074/jbc.M110.163105.PubMedPubMed CentralView ArticleGoogle Scholar
  68. Smith AB, Lopez-Villarejo J, Diago-Navarro E, Mitchenall LA, Barendregt A, Heck AJ, Lemonnier M, Maxwell A, Diaz-Orejas R: A common origin for the bacterial toxin-antitoxin systems parD and ccd, suggested by analyses of toxin/target and toxin/antitoxin interactions. PLoS One. 2012, 7 (9): e46499-10.1371/journal.pone.0046499.PubMedPubMed CentralView ArticleGoogle Scholar
  69. Ramage HR, Connolly LE, Cox JS: Comprehensive functional analysis of Mycobacterium tuberculosis toxin-antitoxin systems: implications for pathogenesis, stress responses, and evolution. PLoS Genet. 2009, 5 (12): e1000767-10.1371/journal.pgen.1000767.PubMedPubMed CentralView ArticleGoogle Scholar
  70. Fiebig A, Castro Rojas CM, Siegal-Gaskins D, Crosson S: Interaction specificity, toxicity and regulation of a paralogous set of ParE/RelE-family toxin-antitoxin systems. Mol Microbiol. 2010, 77 (1): 236-251. 10.1111/j.1365-2958.2010.07207.x.PubMedPubMed CentralView ArticleGoogle Scholar
  71. Lee SK, Chou HH, Pfleger BF, Newman JD, Yoshikuni Y, Keasling JD: Directed evolution of AraC for improved compatibility of arabinose- and lactose-inducible promoters. Appl Environ Microbiol. 2007, 73 (18): 5711-5715. 10.1128/AEM.00791-07.PubMedPubMed CentralView ArticleGoogle Scholar
  72. Amitai S, Kolodkin-Gal I, Hananya-Meltabashi M, Sacher A, Engelberg-Kulka H: Escherichia coli MazF leads to the simultaneous selective synthesis of both “death proteins” and “survival proteins”. PLoS Genet. 2009, 5 (3): e1000390-10.1371/journal.pgen.1000390.PubMedPubMed CentralView ArticleGoogle Scholar
  73. Sambrook J, Russell DW: Molecular cloning. A laboratory manual. 2001, Cold Spring Harbor, N. Y: Cold Spring Harbor Laboratory PressGoogle Scholar
  74. Schagger H: Tricine-SDS-PAGE. Nat Protoc. 2006, 1 (1): 16-22. 10.1038/nprot.2006.4.PubMedView ArticleGoogle Scholar

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