• Loading metrics

A Toxin–Antitoxin System Promotes the Maintenance of an Integrative Conjugative Element

  • Rachel A. F. Wozniak,

    Affiliations Channing Laboratory, Brigham and Women's Hospital, Harvard Medical School, Boston, Massachusetts, United States of America, Howard Hughes Medical Institute, Chevy Chase, Maryland, United States of America, Program in Genetics, Tufts University School of Medicine, Boston, Massachusetts, United States of America

  • Matthew K. Waldor

    Affiliations Channing Laboratory, Brigham and Women's Hospital, Harvard Medical School, Boston, Massachusetts, United States of America, Howard Hughes Medical Institute, Chevy Chase, Maryland, United States of America, Program in Genetics, Tufts University School of Medicine, Boston, Massachusetts, United States of America

A Toxin–Antitoxin System Promotes the Maintenance of an Integrative Conjugative Element

  • Rachel A. F. Wozniak, 
  • Matthew K. Waldor


SXT is an integrative and conjugative element (ICE) that confers resistance to multiple antibiotics upon many clinical isolates of Vibrio cholerae. In most cells, this ∼100 Kb element is integrated into the host genome in a site-specific fashion; however, SXT can excise to form an extrachromosomal circle that is thought to be the substrate for conjugative transfer. Daughter cells lacking SXT can theoretically arise if cell division occurs prior to the element's reintegration. Even though ∼2% of SXT-bearing cells contain the excised form of the ICE, cells that have lost the element have not been detected. Here, using a positive selection-based system, SXT loss was detected rarely at a frequency of ∼1×10−7. As expected, excision appears necessary for loss, and factors influencing the frequency of excision altered the frequency of SXT loss. We screened the entire 100 kb SXT genome and identified two genes within SXT, now designated mosA and mosT (for maintenance of SXT Antitoxin and Toxin), that promote SXT stability. These two genes, which lack similarity to any previously characterized genes, encode a novel toxin-antitoxin pair; expression of mosT greatly impaired cell growth and mosA expression ameliorated MosT toxicity. Factors that promote SXT excision upregulate mosAT expression. Thus, when the element is extrachromosomal and vulnerable to loss, SXT activates a TA module to minimize the formation of SXT-free cells.

Author Summary

Integrative and conjugative elements (ICEs) are a diverse group of mobile genetic elements found in many bacteria. These elements integrate into the host chromosome as well as excise and transfer to other bacteria. SXT, an ICE that encodes resistances to multiple antibiotics, is currently present in most clinical isolates of V. cholerae, the cause of cholera. Cells in which SXT is excised can potentially lose the ICE if cell division occurs prior to its re-integration, but explorations of mechanisms that promote ICE maintenance have received almost no attention. Using a positive selection-based strategy to detect SXT loss, we found that loss of this ICE was very rare (1 in 107 cells). Two genes, mosAT, that lack similarity to genes of known function were found to promote SXT maintenance. We show that MosT blocks cell growth in the absence of SXT and its activity can be neutralized by MosA. Thus, these genes encode a functional toxin–antitoxin (TA) system. When SXT is extrachromosomal and vulnerable to loss, mosAT expression increases, minimizing the formation of SXT-free cells. The activity of mosAT may contribute to the maintenance of antibiotic resistance in bacterial populations.


Integrating and conjugative elements (ICEs) are a class of self-transmissible mobile genetic elements that contribute to horizontal gene exchange among bacteria [1]. With our increasing knowledge of bacterial genomes, ICEs and putative ICEs have been identified in the chromosomes of many gram-positive and gram-negative bacteria [1][7]. ICEs have some features in common with plasmids and bacteriophages, other classes of mobile genetic elements that have been the subjects of more study. Like many temperate bacteriophages, ICEs integrate into and replicate with the host chromosome. However, like conjugative plasmids, ICEs encode DNA processing and type IV secretion machinery that enables their conjugative transfer from donor to recipient cells. ICEs excise from the host chromosome to form an extra-chromosomal circular molecule that is thought to be the substrate for conjugative transfer. Although the excised circular ICE form is presumed to undergo rolling-circle replication concomitant with its transfer from donor to recipient cell, ICEs, unlike plasmids, are not thought to be ordinarily capable of autonomous replication. In addition to diverse integration, excision and conjugation systems, ICEs encode a variety of additional properties including resistance to antibiotics [8][10], nitrogen fixation [11], and degradation of aromatic compounds [12].

SXT is a ∼100 Kb ICE originally discovered in a clinical isolate of the cholera pathogen, Vibrio cholerae [13]. SXT and closely related ICEs encode resistances to antibiotics such as sulfamethoxazole and trimethoprim that have previously been useful for the treatment of cholera. In the past 15 years, SXT-related ICEs have become widespread in clinical V. cholerae isolates in Asia and Africa [14]. SXT-related ICEs have also been isolated from other bacterial species; for example, R391, an Inc J element derived from Providencia rettgeri [15], was found to be genetically and functionally highly similar to SXT [8],[16],[17]. Currently, there are more than 25 known members of the SXT/R391 family of ICEs [14]. These ICEs are all thought to consist of a conserved set of core genes that mediate the elements' integration, excision, conjugation and regulation [18]. Besides the conserved core genes, these ICEs also contain element-specific genes, conferring attributes such as resistance to heavy metals or antibiotics; however, the function of most non-core SXT genes remains unknown.

All SXT/R391 family ICEs encode nearly identical tyrosine recombinases (Int) that mediate the integration of the respective ICEs within the prfC locus in the host chromosome. Int mediates the site-specific recombination between a site (attP) found in the circular form of the ICE and a site (attB) found near the 5′ end of prfC. In addition, these ICEs all encode similar Xis proteins, which act along with Int to promote the elements' excision from the chromosome. Excision occurs by Int-mediated recombination between short sequences found at the right and left ends of the integrated element, yielding the extrachromosomal circular form of the ICE [19]. Xis functions as a recombination directionality factor (RDF), promoting SXT excision and inhibiting its integration [20].

SXT transfer functions are not constitutively expressed. An SXT-encoded repressor, SetR, ordinarily limits SXT transfer. SetR, a homologue of the lambda phage repressor, cI, represses the expression of SetC and SetD, transcription factors that activate expression of int and the tra operons that encode the proteins required for SXT's conjugative transfer [18],[21],[22]. DNA-damaging agents, including certain antibiotics, increase the frequency of SXT transfer by alleviating SetR repression of setDC expression, probably by promoting RecA-dependent SetR autoproteolysis [22].

In host cells that contain an ICE, there is an equilibrium between the integrated and excised circular ICE forms. For example, in the case of E. coli containing SXT, we found that ∼2% of cells in the population harbored excised SXT, detected as an amplifiable chromosomal attB site by quantitative PCR [20]. SXT excision from the chromosome poses a potential threat to the element's stability: if the host divides while SXT is extrachromosomal, the element may not be passed to a daughter cell. Our anecdotal observations suggest that cells rarely if ever lose SXT raising the possibility that this ICE may encode mechanisms to promote its maintenance. To date, there have been no systematic studies of mechanisms that promote ICE maintenance. Here, we developed a positively selectable reporter of SXT loss to begin to explore the environmental and genetic factors that influence this ICE's stability in E. coli. Using this reporter, SXT loss was detected in 1×10−7 cells. Excision appears necessary for loss, and factors influencing the frequency of excision altered the frequency of SXT loss. We screened the entire 100 kb SXT genome and identified two genes, which lack similarity to genes of known function that promote SXT maintenance. These genes, designated mosA and mosT, encode a toxin-antitoxin (TA) system. We found that factors that promote SXT excision also augment mosAT expression. Thus, when the element is extrachromosomal and vulnerable to loss, SXT activates a TA module to minimize formation of SXT-free cells.


A Positively Selectable Reporter of SXT Loss

During serial passage of SXT-bearing strains without selection for SXT-encoded markers, we never detected cells that have lost this ICE, suggesting that SXT is stably maintained in the host population. Given the apparently low frequency of SXT loss, an E. coli reporter strain was designed to allow positive selection of rare cells that have lost SXT (Figure 1). To construct this strain, the Lac repressor, lacIQ, was introduced into an innocuous location in SXT (between traG and s079) while the native lacI was deleted from the chromosome. Additionally, a spectinomycin (Spec) resistance cassette under the control of the lac promoter was introduced into the gal locus in the chromosome (Figure 1). Therefore, in the presence of SXT (and therefore lacIQ), cells are sensitive to spectinomycin. If SXT (and lacIQ) are lost, cells become resistant to spectinomycin. As a result, even very rare cells lacking SXT can be detected as Spec-resistant colony forming units (cfu). Once Spec-resistant cfu are identified, they can subsequently be screened for the presence of SXT-encoded antibiotic resistances, such as chloramphenicol, to confirm SXT loss.

Figure 1. Schematic of a positively selectable reporter of SXT loss.

SXT containing lacIQ was introduced into a lacI E. coli host containing Plac-aad7 (a spectinomycin-resistance gene). If SXT (and lacIQ) is lost, the cells become SpecR. The black diamond represents the site of insertion for a fragment containing lacIQ (pFRTIq), thick black arrows represent ORFs, and the thin black line indicates the approximate location of the Δ9 deletion. Abbreviations: tet = tetracycline resistance gene, kan = kanamycin resistance gene, int = integrase, prfC = site of SXT insertion. Figure not to scale.

Detectable SXT Loss Is Rare

Loss of SXT from the E. coli reporter strain described above was detected at a very low frequency. After 15 hours of growth (∼20 generations) without selection for SXT-encoded markers, only ∼1×10−7 cfu were Spec-resistant and Cm-sensitive, indicating that they had lost SXT (Figure 2A). Similar extremely low levels of SXT loss were observed in exponential and in stationary phase cultures (data not shown), suggesting that culture growth phase does not influence SXT loss. This apparently very low frequency of SXT loss explains why we did not previously detect loss in replica-plating based screens for cells that lost resistance to SXT-encoded antibiotic markers. To confirm that SXT loss was not accompanied by heritable changes in the host chromosome, SXT was re-introduced into the reporter strain that had previously lost this ICE. SXT was lost from this re-constituted SXT loss reporter strain at approximately the same frequency as the original reporter (compare the first bars in Figure 2A and 2B), suggesting that loss of the element was not associated with mutations in the host chromosome.

Figure 2. Influence of genetic factors on the frequency of SXT loss.

The frequency of SXT loss was calculated as the ratio of SpecRCmS cfu / total cfu after 15 hour of growth. A) Factors that influence the frequency of SXT excision alter the frequency of SXT loss. The black diamonds indicate that the result is statistically different (p<0.05) than the result shown in the first column for the wild type reporter. The * signifies that the result was below the limit of detection which was ∼1×10−8. pXis and pXis-R harbor arabinose-inducible xis or its reverse complement respectively. B) SXT loss is not accompanied by heritable changes that influence maintenance of SXT. The ‘current SXT genotype’ refers to the ICE introduced into the host that lost the ICE designated as ‘previous SXT genotype’.

Excision and Loss

To begin to explore the relationship between SXT loss and its excision from the chromosome, we assessed the frequency of SXT excision in our reporter strain using quantitative PCR. In this assay, the amount of attB, which is only generated if SXT excises from the chromosome, is compared to the amount of a stable chromosomal locus (the 3′end of prfC), as described in Burrus and Waldor [20]. We found that SXT excises in 3–4% of cells in the population, a frequency that is nearly 100,000 times the frequency of detectable SXT loss (Table 1). SXT excision may routinely be followed by its re-integration. Furthermore, there may be mechanisms for either preventing DNA replication/cell division when SXT is excised and/or selecting against cells that have lost SXT. Overall, it appears that excision events are only rarely associated with formation of cells that can grow despite losing SXT; however, these numbers may underestimate the true extent of SXT loss if there is selection against such cells.

Table 1. Comparison of SXT excision and loss frequencies.

Since the SXT integrase is required for the element's excision from the chromosome [19],[20], we deleted the int gene from the SXT loss reporter strain to test if SXT loss requires its excision. SXT loss was never observed in the Δint SXT strain (Figure 2A) suggesting, as expected, that SXT excision is required for its loss. However, it is important to note that the limit of detection for this assay is ∼1×10−8, and thus can only conclude that SXT loss is reduced at least 10-fold in the Δint background.

There appears to be some additional correlation between the frequency of SXT excision and its loss. In a recA background, where SXT excision is reduced (data not shown), there was a statistically significant reduction in SXT loss (Figure 2A). Conversely, increased SXT excision promoted its loss. Overexpression of Xis, the SXT recombination directionality factor (RDF), which increases the frequency of excised SXT (unpublished observations), resulted in an ∼500-fold increase in SXT loss (Figure 2A, pXis bar). A control plasmid containing xis in the reverse orientation (pXisR) did not alter SXT loss (Figure 2A). As an RDF, Xis could promote SXT loss by both promoting its excision and inhibiting its reintegration into the host chromosome.

Conjugation Does Not Lead to SXT Loss

Using the SXT loss reporter strain as a donor in conjugation experiments, we were able to address a longstanding question regarding SXT: do donors lose this ICE during conjugation? Following a 2 hour mating between the SXT loss reporter with an E. coli recipient, cells were plated on selective media to score for the number of donors, recipients, and exconjugants, as well as loss of SXT from the donor. As a control, the donor was grown by itself in identical conditions. As shown in Table 2, the frequency of exconjugant formation in this experiment was more than four orders of magnitude greater than the frequency of detectable SXT loss from the donor strain. Furthermore, the frequencies of SXT loss from the donor that was mixed with the recipient and the donor grown by itself under identical conditions were fairly similar. Although not statistically significant, there appears to be less loss of SXT when the donor was mixed with the recipient (Table 2). Together these observations suggest that donors do not lose SXT during conjugation and that a copy of SXT re-integrates into the donor chromosome following transfer of the ICE to the recipient.

Identification of SXT Genes That Promote Its Maintenance

Given the very low frequency of SXT loss, we hypothesized that SXT contains genes that promote its maintenance in the host. We took advantage of a set of previously constructed SXT deletion mutants [18] and constructed new deletion mutants to screen for regions of this ICE's genome that contribute to its stability. The features of the SXT loss reporter as outlined in Figure 1 were introduced into 11 SXT deletion mutants spanning the entire SXT genome, yielding 11 new SXT loss reporter strains (Table 3). Each of the new reporters was tested for SXT loss and the findings from these experiments are summarized in Table 3.

Nearly all of the mutants tested exhibited rare loss of SXT, very similar to the loss frequency for wild type SXT. Several mutants (Δ3, Δ4, Δ8 and ΔE) contained deletions in genes required for conjugative transfer [18]; however, these mutants did not exhibit decreased SXT loss (Table 3) as would be expected if conjugation promoted SXT loss. Two deleted regions, Δ2 and Δ10, primarily consisted of predicted open reading frames of unknown or conserved hypothetical function, but these regions did not contain genes important for SXT maintenance (Table 3). Finally, two deletions that might have been suspected to influence SXT stability, Δ1 and Δ7, did not. The Δ1 deletion includes several transposases but deletion of this region did not promote SXT instability. The two genes deleted from the Δ7 mutant, s044-45, were previously proposed to function as a toxin-antitoxin module in SXT based on homology to a TA pair encoded in the Paracoccus aminophilus plasmid pAMI2 [23]. Our observation that the Δ7 mutant did not exhibit increased SXT loss argues against the idea that these genes encode a functional TA module in SXT.

However, deletion of the 8 genes in the Δ9 mutant, which spans the region from s052 to traN, resulted in growth of markedly more colonies that lacked SXT (∼1×10−4), than observed to lack wt SXT (∼1×10−7) (Table 3 and Figure 3B). Five of the eight genes (see Figure 3A) in this deletion (traC, trsF, traW, traU, traN) are important for conjugative transfer of SXT. s054 encodes a homologue of a disulfide bond isomerase-related protein and s052 and s053 are currently classified as hypothetical genes with no known function, characterized homologues, or recognizable motifs. We constructed smaller deletions within the s052-traN region to pinpoint those gene(s) that account for the increased loss observed for the Δ9 mutant. As expected, ΔA, which only removed genes implicated in conjugative transfer, did not alter SXT stability (Figure 3B); deletion of s054 did not influence SXT stability either. However ΔB, which contains s052 and s053, resulted in a similar frequency of loss as the Δ9 mutant. Finally, deletion of s053 alone was sufficient to recapitulate the Δ9 phenotype (Figure 3B). It is important to note that while s052 and s053 could be deleted together, s052 could not be deleted in the presence of s053. From this point on, for reasons that will become clear below, s052 and s053 are referred to as mosA and mosT, respectively, for maintenance of SXT (Antitoxin, Toxin).

Figure 3. Genetic analysis of loss of mosT SXT.

A) Schematic of the region deleted from Δ9 SXT. Black arrows represent ORFs, thin black arrows represent the deletions studied below. B) Frequency of loss of the indicated mutant SXT. C) Influence of mosT expression in trans on the stability of mosT SXT. All cultures were grown in the presence of 0.02% arabinose for 15 hr. Black diamond represents a statistically significant (p<.05) result compared to loss in the presence of pBAD33. D) Loss of mosT SXT is influenced by factors affecting SXT excision. All cultures were grown for 15 hr except as noted. Black diamonds represent a statistically significant (p<0.05) result compared to the mosT SXT grown for 15 hr. The * signifies that the result was below the limit of detection which was ∼1×10−8. aLoss was calculated following 3 hours of growth in an early log phase culture.

MosT Acts In Trans and Appears to Function following SXT Excision

We confirmed that the elevated frequency of loss of mosT SXT was due to the absence of mosT and not to a secondary mutation on the chromosome or in SXT in several ways. First, a mosT SXT as well as a wild-type SXT were reintroduced into a strain that had previously lost mosT SXT. In these two new strains, the frequency of loss of the respective ICEs was very similar to that observed in their original hosts (compare Figure 2B, 3rd and 4th bars vs. Figure 2A 1st bar and 3B 5th bar respectively), demonstrating that the high frequency of mosT SXT loss is not due to changes in the chromosome of its original host. Furthermore, the frequency of loss of mosT SXT from an E. coli strain that had previously lost wild type SXT was approximately the same as observed in the original host (Figure 2B, 2nd bar vs 3B, 5th bar), lending support to the idea that the elevated frequency of loss of mosT SXT is linked to this ICE. Finally, introducing the mosT deletion into a wild type E. coli SXT loss reporter strain, using either P1 transduction or λ Red-based technology [24] resulted in mosT SXT strains that had frequencies of mosT SXT loss that were the same as observed in our original mutant (data not shown). Together, these observations link the elevated frequency of mosT SXT loss to the absence of mosT.

To test whether mosT could act in trans to complement the elevated loss phenotype of mosT SXT, we constructed an arabinose-inducible version of mosT in the low copy vector pBAD33. Loss of mosT SXT was measured under inducing conditions in the presence of either the mosT-expression vector, pMosT, pBAD33 (empty vector), or pMosT', a pMosT derivative that was engineered to contain a stop codon in the 11th codon of mosT. As shown in Figure 3C, expression of mosT from pMosT restored the stability of mosT SXT to levels observed in wild type SXT. In contrast, pMosT' did not alter the ICE's stability (compare 1st and 3rd bars Figure 3C). These observations suggest that mosT encodes a protein that promotes SXT stability.

To begin to explore how mosT influences SXT stability, we looked for conditions that alter the loss of mosT SXT. As with wild type SXT, the frequency of mosT SXT loss was not altered by growth phase (Figure 3D). MosT appears to act after SXT excises from the chromosome, since the frequency of mosT SXT excision was almost identical to that of wild type SXT (Table 1). Consistent with this idea, we found that mosT SXT loss was responsive to factors that influence SXT excision (Figure 3D) as observed above for wild type SXT. For example, loss of mosT SXT was abolished when int was deleted from mosT SXT and was reduced when a recA mutation was introduced into the host chromosome (Figure 3D and data not shown). Conversely, increasing mosT SXT excision by overexpression of Xis resulted in a significant increase in mosT SXT loss, whereas the control vector, pXis-R, did not alter mosT SXT loss (Figure 3D). Overall, the effects of mosT and xis appear to be independent, providing support for the idea that mosT likely acts after excision.

MosT Inhibits Growth of E. coli and V. cholerae

Our observation that s052 (mosA) could not be deleted in the presence of s053 (mosT) but that mosT could be deleted regardless of the presence of mosA suggested the possibility that mosT and mosA might comprise a toxin-antitoxin (TA) pair. TA pairs were originally described in plasmids but are now known to be present in many chromosomes as well [25],[26]. The toxin components of plasmid-borne TA modules are more stable than their cognate antitoxins; thus, cells that fail to inherit plasmids and can no longer synthesize antitoxin are thought to die or have impaired growth due to residual toxin activity [25],[27]. Several functions of chromosomal TA modules, including stress responses [28],[29] and stabilization of large chromosomal regions [30],[31], have been proposed. Consistent with the idea that mosT encodes a toxin, we found that mosT could only be cloned downstream of the arabinose-inducible promoter PBAD in the presence of glucose, which represses PBAD [32]. Furthermore, in the presence of arabinose, growth of E. coli harboring this plasmid-borne inducible mosT (pMosT) was severely impaired. There was minimal increase in culture OD600 following MosT induction (Figure 4A) and induction caused cfu to drop by several orders of magnitude (Figure 4B). Together, these data suggest that mosT over-expression is toxic to E. coli and V. cholerae (data not shown).

Figure 4. MosT inhibits E. coli growth and its toxicity can be neutralized by MosA.

Growth kinetics of E. coli strains CAG18439 (A and B), CAG18439 containing mosAT SXT (C) and CAG18439 containing wild type SXT (D). These strains, which harbored arabinose-inducible mosT and mosA, (pMosT or pMosA respectively) or control vectors, (pBAD33 and pBAD18), were grown in either 0.2% glucose (solid lines) or 0.02% arabinose (dashed lines).

MosA Can Neutralize MosT

Over-expression of MosT caused similar growth inhibition in E. coli lacking SXT (Figure 4A) and E. coli harboring mosAT SXT (Figure 4C), but had no effect on growth of E. coli harboring wild type SXT (Figure 4D), suggesting that mosA can neutralize the toxic effects of over-expressed MosT. To assess this possibility, we generated an arabinose-inducible mosA construct (in pMosA1). However, we were unable to demonstrate mosA neutralizing activity using this initial construct. Subsequent studies revealed that the putative mosA open reading frame was mis-annotated. 5′ RACE experiments to identify the +1 nucleotide of the mosA transcript (Figure 5B) suggested that the true mosA transcript begins upstream from the original annotation (Figure 5). Promoter and ORF predictions (BProm, FGENESB; for mosA were consistent with the 5′ RACE results. We constructed a new arabinose-inducible mosA vector (pMosA) that included the entire mosA transcript; induction of mosA expression from this vector completely blocked the growth inhibitory effect of MosT in E. coli or E. coli harboring mosAT SXT (Figure 4A–C). An empty pBAD18 vector control did not diminish mosT toxicity (Figure 4A–C). Together, these findings are consistent with the idea that mosT and mosA encode a toxin and antitoxin respectively.

Figure 5. 5′RACE analysis of mosA transcription start site.

A) Schematic of mosA transcription start site based on the 5′ RACE results shown in B). The +1 refers to the start of transcription as defined by the DNA sequence of the 5′RACE product obtained using primer A (small black arrow). The length of the PCR product is indicated. Black arrows represent ORFs as predicted using bioinformatics; the previously annotated s052 start codon is indicated. B) Shows a 1% agarose gel of the product of 5′RACE reaction using primer A.

Excision Promotes mosAT Transcription

To begin to explore the factors that promote expression of the mosAT locus, we inserted a promoterless lacZ gene downstream of the mosA promoter, leaving intact copies of the wild type genes (Figure 6A). mosA and mosT are likely co-transcribed since the two genes overlap, additional 5′ RACE experiments and Northern analyses are consistent with this idea (data not shown), and other characterized TA loci are operons [33],[34]. There was relatively weak basal activity of the mosA promoter measured in an overnight culture of the reporter strain (Figure 6B) and no detectable β-galactosidase activity in an isogenic control strain lacking a lacZ fusion (data not shown).

Figure 6. Influence of Xis and SetCD on mosA expression.

A) Schematic of chromosomal mosA:: lacZ transcription reporter within the mosAT locus. Thick black arrows represent ORFs as predicted by bioinformatics and the thin arrow represents the predicted location of the mosA promoter. B, D) β-galactosidase activities of the chromosomal mosA::lacZ fusion in CAG18439 containing wt SXT (B) or in CAG18439 containing Δint SXT (D) along with the indicating expression vectors. C) β-galactasidase activities from a plasmid-borne mosA-lacZ fusion (in pPmosA) in the indicated strains. All β-galactasidase measurements were conducted on 15 hr cultures and the results shown are the means and standard deviation from at least 9 independent cultures.

We explored if the low activity of the mosA promoter was due to repression by MosA, since such autorepression has been observed for several other TA loci [33],[34]. The β-galactosidase activity derived from a plasmid-borne mosA promoter-lacZ fusion (in pPmosA) was found to be ∼10-fold higher in the absence vs. the presence of SXT, suggesting that SXT encodes a repressor of mosA (Figure 6C). Furthermore, reporter activity was elevated to a similar extent in SXT and mosAT SXT E. coli strains, and reduced to comparable levels in strains containing wild type and mosT SXT (Figure 6C). Together, these data indicate that MosA can function independently of MosT to repress its own expression.

Since SXT is vulnerable to loss following its excision, we tested if factors that promote SXT excision also promote mosAT expression. Overexpression of Xis from the arabinose-inducible promoter in pXis augmented the activity of the chromosomal mosA-lacZ fusion more than 4-fold (Figure 6B), whereas addition of arabinose to the reporter strain harboring the control vector, pXis-R did not alter β-galactosidase activity (Figure 6B). Furthermore, overexpression of SetC and SetD, the key transcription activators that control SXT transfer, increased transcription from the mosA promoter (Figure 6B). These observations suggest that expression of mosAT is linked to conditions, such as production of Xis, SetC and SetD, that promote SXT excision. Furthermore, elevations in SXT copy number that may occur with excision [20] would increase mosAT gene dosage, providing more template for their transcription.

To test if SXT excision was essential for Xis-mediated induction of mosA transcription, the chromosomal mosA-lacZ fusion was introduced into an int SXT background. In this context, overexpression of Xis still increased expression of mosA (∼2.5 fold) but not to the same extent as in the wt SXT background (∼4.0 fold) (compare Figure 6B and 6D). Since Xis can augment mosA expression independently of SXT excision, it is possible that this RDF can directly influence transcription, as described for several other RDFs [35].


When integrated in a host genome, SXT and other ICEs are stably maintained, as they are replicated along with the chromosome. However, once excised from the host genome, even with some degree of replication, ICEs are at risk of being lost if cell division occurs prior to element re-integration. Without mechanisms to promote SXT reintegration and/or prevent growth of daughter cells lacking SXT, cells that have lost SXT should be detectable, since SXT excises from the chromosome in more than 1 in 100 cells. Yet our previous attempts to identify cells that have lost SXT using replica plating-based assays did not reveal any SXT loss. In light of our current work, our previous failure to detect SXT loss is understandable. Using the positive selection-based strategy developed here, we detected SXT loss in only 1 in 107 cells. Furthermore, SXT appears to be lost after the ICE excises from the chromosome, since loss doesn't occur when SXT cannot excise. Two genes that lack similarity to genes of known function were found to promote SXT maintenance, although they do not influence SXT excision frequency or conjugation frequency (data not shown). These 2 genes, mosT and mosA, function as a toxin-antitoxin system. Exogenous expression of mosT greatly impaired cell growth, and mosA expression ameliorated MosT toxicity. Basal expression of mosAT is quite low; however, factors that promote SXT excision, like Xis and SetCD, augment mosAT expression. Thus, our observations suggest that when the element is extrachromosomal and vulnerable to loss, SXT activates a TA module to minimize the formation of SXT-free cells.

Comprehensive screens for genes that promote ICE maintenance have not previously been carried out and explorations of mechanisms that promote ICE stability have received little attention. To date, there has been only one report of a gene that promotes the stability of an ICE. Qui et al. found that the P. aeruginosa ICE PAPI-1 contains a homologue of the plasmid and chromosome partitioning gene soj (parA). They demonstrated that deletion of the soj homologue from PAPI-1 resulted in complete loss of PAPI-1 from P. aerguinosa [3]. The mechanism by which Soj promotes PAPI-1 maintenance remains to be elucidated; however, it is unlikely that Soj functions as a toxin like MosT.

Prior to our study, TA systems have not directly been shown to promote ICE maintenance. Dziewitt et al. proposed that s044 and s045, two SXT genes with similarity to TA genes found in the Paracoccus aminophilus plasmid pAMI2, promote SXT stability [23]. They found that these two SXT genes augmented the stability of a heterologous unstable plasmid [23]; however, our observation that deletion of s044 and s045, (in the Δ7 SXT mutant), did not result in elevated SXT loss argues against the idea that these genes influence SXT maintenance.

Unlike previously described TA loci, mosAT are part of a dynamic mobile genetic element that is predominantly found integrated in the chromosome but that can also exist in an extrachromosomal form. As demonstrated by the lacZ transcriptional fusion data (Figure 6), mosAT has low basal transcription due to autorepression by MosA, as described in several other TA loci [33],[34]. Therefore, mosAT likely remains in a repressed state while SXT is integrated in the host chromosome. It is unknown whether these genes have physiologic function when SXT is integrated. However, mosAT appear to be derepressed by the actions of Xis and SetC and SetD, proteins that promote SXT excision. Thus, the activity of mosAT may be limited to the time when SXT is extrachromosomal and vulnerable to loss. Since our current studies are population-based, a more refined understanding of the timing of mosAT expression in relation to SXT excision will be possible if we can develop assays to monitor mosAT expression and SXT excision in single cells.

There is controversy about the ordinary physiologic role of toxins that are part of chromosomal toxin antitoxin systems. Some propose that these toxins' physiologic function is to kill host cells whereas others propose that toxins function to limit metabolic processes such as protein synthesis as part of stress responses [29],[36]. MosT could act in either fashion to promote the maintenance of the excised form of SXT. Assuming that mosAT is an operon and MosA is less stable than MosT, then cells from which SXT is absent should be subject to the effects (presumably death) of MosT, similar to many plasmid-encoded toxins that are thought to kill host cells that fail to inherit the plasmid. However, it also possible that MosT is active prior to loss of SXT (e.g., via preferential degradation of MosA, as described for the RelB anti-toxin, [29]), and that it stalls cell growth until SXT has reintegrated and MosT's effects can be turned off. If so, MosT's effects would need to be reversible, so that the cell could resume growth upon SXT re-integration. Future studies to discover the MosT target and its mechanism(s) of action may enable discrimination between these possibilities.

If mosAT guards against SXT loss when the element is extrachromosomal, as we propose, then linking expression of these genes to SXT excision makes sense. There are several reports of excised forms of mobile elements increasing expression of genes that act on the excised (and often circular) forms of the elements. For example, expression of the PAPI-1 soj gene is increased in the circular form of the ICE by the joining of a promoter located on the 3′ end of the integrated element to soj (which is found at the 5′ end of the ICE) when PAPI-1 circularizes [3]; a similar mechanism drives the expression of genes required for conjugative transfer of Tn916 [37]. The mosAT locus is found near the middle of the SXT genome, so generation of a promoter through SXT circularization cannot directly influence mosAT expression. Instead, we found that factors that promote SXT excision including Xis and SetC and SetD augmented mosAT expression. Xis may act, at least in part, directly at the mosA promoter to increase mosAT expression, since Xis augmented mosA expression even when SXT was unable to excise. Other RDFs such as the Cox proteins HP1 and P2, have also been shown to act as transcription factors [38]. Currently the factors that govern Xis expression and activity are not known. It is also unclear at this point whether SetC and SetD act directly to promote mosAT expression.

Although mosAT expression and function appears to be highly adapted to SXT, these genes are not found in all SXT/R391 family ICEs. A few of these elements, including R391, an ICE originally derived from an African Providencia rettgeri strain [8],[15], and ICEVchMex1, an ICE derived from a Mexican environmental V. cholerae strain [39], lack mosAT. The mosAT locus is found in one of the SXT ‘hot-spots’, regions of hypervariability that are not conserved among SXT/R391 family elements (Beaber et al 2002). As such, mosAT does not represent a universal strategy for the maintenance of the stability of SXT/R391 family ICEs. Preliminary studies suggest that R391 is only slightly less stable than SXT, raising the possibility that R391, like SXT, has acquired additional genes to promote its maintenance.

A recent BLASTP search revealed many proteins with sequences similar to MosA and MosT in gram-negative bacteria. Overall, MosT exhibited greater conservation and contains a widely conserved domain of unknown function (DUF1814) present in both bacteria and archaea. However, MosA homologues were routinely found adjacent to MosT homologues. In total, there were 5 proteins whose amino acid sequences are identical or nearly identical to MosT from SXT and 30 proteins whose amino acid sequences bear significant similarity to MosT (E values less than 4×10−50). Proteins with near identity to MosT, from several recently sequenced V. cholerae strains and from Proteus mirabilis HI4320, appear to be part of previously unannotated SXT/R391 family elements. However, with one exception, the proteins with significant similarity to MosT appear to be encoded by chromosomes that do not contain an SXT/R391 family ICE, raising the possibility that they function to promote the stability of a non-SXT-related ICE or perhaps perform another function for the host genome. There is an octopine type Ti plasmid from Agrobacterium tumefaciens that contains genes with similarity to mosA and mosT, suggesting that these genes may be able to promote the stability of plasmids as well as ICEs. Overall, the presence of mosAT-like genes outside of SXT/R391 family of ICEs suggests that these genes have been and perhaps remain transmissible.

Materials and Methods

Media, Growth Conditions, and Growth Assays

Bacterial cultures were routinely grown in Luria-Burtani (LB) broth at 37°C in a shaking incubator. Antibiotics were used at the following concentrations: ampicillin, 100 µg/ml; chloramphenicol, 20 µg/ml; kanamycin, 50 µg/ml; nalidixic acid, 40 µg/ml; sulfamethoxazole, 160 µg/ml; trimethoprim, 32 µg/ml; tetracycline, 6 µg/ml; and spectinomycin 30 µg/ml. 5-bromo-4-chloro-3indolyl-beta-D-galactopyranoside (X-gal) was used at 60 µg/ml, arabinose at 0.02% (vol/vol) and glucose at 0.2% (vol/vol). Strains were maintained at −80°C in LB containing 20% (vol/vol) glycerol.

For the growth curves presented in Figure 4, cultures were initially grown overnight in the presence of appropriate antibiotics plus 0.2% glucose. The cells were then washed 2× in equal volumes of fresh LB and then diluted 1∶1000 into LB plus 0.02% arabinose or 0.2% glucose. Each culture was tested in triplicate by applying 200 µl to each of 3 wells of a 96-well culture plate. The cultures were then grown in a Synergy HT microplate reader (BioTek) with shaking at 37°C for10 hours; OD600 measurements were acquired every 20 min. The numbers of colony-forming units were measured by plating serial dilutions of cultures grown under similar conditions on plates containing chloramphenicol and 0.2% glucose.

Strain and Plasmid Construction

A complete list of the strains and plasmids used in this study can be found in Table 4.

In the SXT loss reporter strains, ΔlacI::kn and ΔgalETKM::Placspec were introduced into the respective chromosomal loci using the lambda Red recombination system as described [24]. The PCR product used to create the ΔlacI::kn deletion/insertion was generated using the pKD4 plasmid as a template and primers designed to omit the FRT sites. To generate the Placspec PCR product used to create the ΔgalETKM::Placspec deletion/insertion, first a spectinomycin cassette was cloned into pCRII-TOPO (Invitrogen); then, this fragment along with the upstream lac promoter was used as a template to amplify the Placspec fragment. The structure of the engineered ΔlacI::kn and ΔgalETKM::Placspec loci were each confirmed by several PCR assays. The construct used to insert lacIq into SXT (pFRTIq) was constructed by first cloning lacIq and the FRT sequence (GAAGTTCCTATACTTTCTAGAGAATAGGAACTTC) into the suicide vector pAH162 [40]. A FRT site was also introduced into E. coli CAG18439 carrying SXT immediately downstream of traG using lambda Red-based technology in all strains except ΔD and ΔE. Finally, pFRTIq was introduced into this strain and the Flippase encoded on plasmid pCP20 [24] was used to mediate the integration of pFRTIq into SXT immediately 3′ of traG. In ΔD and ΔE, a FRT site was initially introduced into the site of the deletion and then pECA102 (kindly provided by D.E. Cameron), which contains a modified Flippase, was used to mediate the integration of pFRTIq. The correct insertion of pFRTIq was verified using PCR.

RecA mutants were created by P1 transduction of the recA allele from HK57, an E. coli strain that contains the RecA1 allele linked to slr::Tn10 [41]. Transductants were selected as tetracycline-resistance cfu and the recA mutation was subsequently confirmed by assessing sensitivity to UV exposure.

The arabinose-inducible mosT and mosA expression vectors, pMosT and pMosA, were constructed by amplifying mosT and mosA with flanking restriction sites using PCR and then cloning the PCR products into pBAD33 and pBAD18 [32], respectively. The correct inserts were verified by PCR as well as DNA sequencing.

A chromosomal mosA::lacZ fusion was constructed by initially amplifying a fragment encompassing the predicted mosA promoter. Then, the PCR product was cloned into the suicide vector, pVIK112, which contains a lacZ gene downstream from a multiple cloning site [42]. Integration of the plasmid into the chromosome enabled measurement of mosA promoter activity in the presence of an intact copy of the gene.

pPmosA was created by subcloning the mosA promoter region into the lacZ fusion vector, pCB192 [43] in order to evaluate the expression of the mosA promoter in the absence of SXT.

SXT Loss Calculation

Reporter strains were generally grown for 15 hr in LB and then serial dilutions were plated on agar containing spectinomycin and kanamycin. Approximately 100–500 colonies were subsequently replica plated or patched to agar containing chloramphenicol, a marker carried by SXT, to estimate the false positive rate. The false positive rate was calculated by dividing the number of CmR cfu by the number of SpecR cfu. Thus, the frequency of SXT loss was calculated as (SpecR cfu/Total cfu)*(1-frequency of false positives). All loss assays were repeated a minimum of 6 times. A two-tailed, non-paired T-test was used to assess the statistical difference between SXT loss values. P values≤0.05 were considered statistically different.

Conjugation Assay

Conjugation experiments were conducted as previously described [13]. Briefly, donor and recipient cells were mixed on a LB plate for 2 hours at 37°C. The cells were then resuspended and plated on the appropriate selective media to count the number of donor, recipient and exconjugant cfu. In order to accurately measure loss in the context of mating only, strains were kept on selection for SXT until the start of the experiment. Prior to mixing donor and recipient strains, the cells were washed 2× in fresh LB to remove traces of antibiotics from the liquid media.

Miscellaneous Molecular Biology Methods

DNA manipulations were carried out using standard techniques [44]. Quantitative Real Time PCR assays were conducted as previously described [20] using primers to amplify attB, and a portion of the 3′ region of prfC. DNA sequencing was done by GeneWiz. 5′RACE was conducted as per the manufacturer's instructions (Invitrogen) to determine the start site for mosA transcription. Assays for β-galactosidase activities in overnight cultures were carried out as previously described [45].


We are grateful to Brigid Davis for her insightful comments and suggestions on the manuscript.

Author Contributions

Conceived and designed the experiments: RAFW MKW. Performed the experiments: RAFW. Analyzed the data: RAFW MKW. Wrote the paper: RAFW MKW.


  1. 1. Burrus V, Waldor MK (2004) Shaping bacterial genomes with integrative and conjugative elements. Res Microbiol 155: 376–386.
  2. 2. Churchward G (2008) Back to the future: the new ICE age. Mol Microbiol 70: 554–556.
  3. 3. Qiu X, Gurkar AU, Lory S (2006) Interstrain transfer of the large pathogenicity island (PAPI-1) of Pseudomonas aeruginosa. Proc Natl Acad Sci U S A 103: 19830–19835.
  4. 4. Auchtung JM, Lee CA, Monson RE, Lehman AP, Grossman AD (2005) Regulation of a Bacillus subtilis mobile genetic element by intercellular signaling and the global DNA damage response. Proc Natl Acad Sci U S A 102: 12554–12559.
  5. 5. Pavlovic G, Burrus V, Gintz B, Decaris B, Guedon G (2004) Evolution of genomic islands by deletion and tandem accretion by site-specific recombination: ICESt1-related elements from Streptococcus thermophilus. Microbiology 150: 759–774.
  6. 6. Lin TL, Lee CZ, Hsieh PF, Tsai SF, Wang JT (2008) Characterization of integrative and conjugative element ICEKp1-associated genomic heterogeneity in a Klebsiella pneumoniae strain isolated from a primary liver abscess. J Bacteriol 190: 515–526.
  7. 7. Pembroke JT, Piterina AV (2006) A novel ICE in the genome of Shewanella putrefaciens W3-18-1: comparison with the SXT/R391 ICE-like elements. FEMS Microbiol Lett 264: 80–88.
  8. 8. Boltner D, MacMahon C, Pembroke JT, Strike P, Osborn AM (2002) R391: a conjugative integrating mosaic comprised of phage, plasmid, and transposon elements. J Bacteriol 184: 5158–5169.
  9. 9. Rice LB (1998) Tn916 family conjugative transposons and dissemination of antimicrobial resistance determinants. Antimicrob Agents Chemother 42: 1871–1877.
  10. 10. Whittle G, Shoemaker NB, Salyers AA (2002) The role of Bacteroides conjugative transposons in the dissemination of antibiotic resistance genes. Cell Mol Life Sci 59: 2044–2054.
  11. 11. Sullivan JT, Ronson CW (1998) Evolution of rhizobia by acquisition of a 500-kb symbiosis island that integrates into a phe-tRNA gene. Proc Natl Acad Sci U S A 95: 5145–5149.
  12. 12. Ravatn R, Studer S, Springael D, Zehnder AJ, van der Meer JR (1998) Chromosomal integration, tandem amplification, and deamplification in Pseudomonas putida F1 of a 105-kilobase genetic element containing the chlorocatechol degradative genes from Pseudomonas sp. Strain B13. J Bacteriol 180: 4360–4369.
  13. 13. Waldor MK, Tschape H, Mekalanos JJ (1996) A new type of conjugative transposon encodes resistance to sulfamethoxazole, trimethoprim, and streptomycin in Vibrio cholerae O139. J Bacteriol 178: 4157–4165.
  14. 14. Burrus V, Marrero J, Waldor MK (2006) The current ICE age: biology and evolution of SXT-related integrating conjugative elements. Plasmid 55: 173–183.
  15. 15. Coetzee JN, Datta N, Hedges RW (1972) R factors from Proteus rettgeri. J Gen Microbiol 72: 543–552.
  16. 16. Hochhut B, Beaber JW, Woodgate R, Waldor MK (2001) Formation of chromosomal tandem arrays of the SXT element and R391, two conjugative chromosomally integrating elements that share an attachment site. J Bacteriol 183: 1124–1132.
  17. 17. Beaber JW, Burrus V, Hochhut B, Waldor MK (2002) Comparison of SXT and R391, two conjugative integrating elements: definition of a genetic backbone for the mobilization of resistance determinants. Cell Mol Life Sci 59: 2065–2070.
  18. 18. Beaber JW, Hochhut B, Waldor MK (2002) Genomic and functional analyses of SXT, an integrating antibiotic resistance gene transfer element derived from Vibrio cholerae. J Bacteriol 184: 4259–4269.
  19. 19. Hochhut B, Waldor MK (1999) Site-specific integration of the conjugal Vibrio cholerae SXT element into prfC. Mol Microbiol 32: 99–110.
  20. 20. Burrus V, Waldor MK (2003) Control of SXT integration and excision. J Bacteriol 185: 5045–5054.
  21. 21. Beaber JW, Waldor MK (2004) Identification of operators and promoters that control SXT conjugative transfer. J Bacteriol 186: 5945–5949.
  22. 22. Beaber JW, Hochhut B, Waldor MK (2004) SOS response promotes horizontal dissemination of antibiotic resistance genes. Nature 427: 72–74.
  23. 23. Dziewit L, Jazurek M, Drewniak L, Baj J, Bartosik D (2007) The SXT conjugative element and linear prophage N15 encode toxin-antitoxin-stabilizing systems homologous to the tad-ata module of the Paracoccus aminophilus plasmid pAMI2. J Bacteriol 189: 1983–1997.
  24. 24. Datsenko KA, Wanner BL (2000) One-step inactivation of chromosomal genes in Escherichia coli K-12 using PCR products. Proc Natl Acad Sci U S A 97: 6640–6645.
  25. 25. Zielenkiewicz U, Ceglowski P (2001) Mechanisms of plasmid stable maintenance with special focus on plasmid addiction systems. Acta Biochim Pol 48: 1003–1023.
  26. 26. Pandey DP, Gerdes K (2005) Toxin-antitoxin loci are highly abundant in free-living but lost from host-associated prokaryotes. Nucleic Acids Res 33: 966–976.
  27. 27. Ruiz-Echevarria MJ, Berzal-Herranz A, Gerdes K, Diaz-Orejas R (1991) The kis and kid genes of the parD maintenance system of plasmid R1 form an operon that is autoregulated at the level of transcription by the co-ordinated action of the Kis and Kid proteins. Mol Microbiol 5: 2685–2693.
  28. 28. Kolodkin-Gal I, Engelberg-Kulka H (2006) Induction of Escherichia coli chromosomal mazEF by stressful conditions causes an irreversible loss of viability. J Bacteriol 188: 3420–3423.
  29. 29. Christensen SK, Mikkelsen M, Pedersen K, Gerdes K (2001) RelE, a global inhibitor of translation, is activated during nutritional stress. Proc Natl Acad Sci U S A 98: 14328–14333.
  30. 30. Szekeres S, Dauti M, Wilde C, Mazel D, Rowe-Magnus DA (2007) Chromosomal toxin-antitoxin loci can diminish large-scale genome reductions in the absence of selection. Mol Microbiol 63: 1588–1605.
  31. 31. Magnuson RD (2007) Hypothetical functions of toxin-antitoxin systems. J Bacteriol 189: 6089–6092.
  32. 32. Guzman LM, Belin D, Carson MJ, Beckwith J (1995) Tight regulation, modulation, and high-level expression by vectors containing the arabinose PBAD promoter. J Bacteriol 177: 4121–4130.
  33. 33. Gotfredsen M, Gerdes K (1998) The Escherichia coli relBE genes belong to a new toxin-antitoxin gene family. Mol Microbiol 29: 1065–1076.
  34. 34. Budde PP, Davis BM, Yuan J, Waldor MK (2007) Characterization of a higBA toxin-antitoxin locus in Vibrio cholerae. J Bacteriol 189: 491–500.
  35. 35. Lewis JA, Hatfull GF (2001) Control of directionality in integrase-mediated recombination: examination of recombination directionality factors (RDFs) including Xis and Cox proteins. Nucleic Acids Res 29: 2205–2216.
  36. 36. Engelberg-Kulka H, Amitai S, Kolodkin-Gal I, Hazan R (2006) Bacterial programmed cell death and multicellular behavior in bacteria. PLoS Genet 2: e135.
  37. 37. Celli J, Trieu-Cuot P (1998) Circularization of Tn916 is required for expression of the transposon-encoded transfer functions: characterization of long tetracycline-inducible transcripts reading through the attachment site. Mol Microbiol 28: 103–117.
  38. 38. Esposito D, Wilson JC, Scocca JJ (1997) Reciprocal regulation of the early promoter region of bacteriophage HP1 by the Cox and Cl proteins. Virology 234: 267–276.
  39. 39. Burrus V, Quezada-Calvillo R, Marrero J, Waldor MK (2006) SXT-related integrating conjugative element in New World Vibrio cholerae. Appl Environ Microbiol 72: 3054–3057.
  40. 40. Haldimann A, Wanner BL (2001) Conditional-replication, integration, excision, and retrieval plasmid-host systems for gene structure-function studies of bacteria. J Bacteriol 183: 6384–6393.
  41. 41. Kimsey HH, Dagarag MD, Kumamoto CA (1995) Diverse effects of mutation on the activity of the Escherichia coli export chaperone SecB. J Biol Chem 270: 22831–22835.
  42. 42. Kalogeraki VS, Winans SC (1997) Suicide plasmids containing promoterless reporter genes can simultaneously disrupt and create fusions to target genes of diverse bacteria. Gene 188: 69–75.
  43. 43. Schneider K, Beck CF (1986) Promoter-probe vectors for the analysis of divergently arranged promoters. Gene 42: 37–48.
  44. 44. Sambrook J (2001) Molecular Cloning; Library CSH, editor.
  45. 45. Miller J (1992) A short course in bacterial genetics. Cold Spring Harbor, N.Y.: Cold Spring Harbor Laboratory Press.
  46. 46. Guyer MS, Reed RR, Steitz JA, Low KB (1981) Identification of a sex-factor-affinity site in E. coli as gamma delta. Cold Spring Harb Symp Quant Biol 45 Pt 1: 135–140.
  47. 47. Singer M, Baker TA, Schnitzler G, Deischel SM, Goel M, et al. (1989) A collection of strains containing genetically linked alternating antibiotic resistance elements for genetic mapping of Escherichia coli. Microbiol Rev 53: 1–24.