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Summary

  1. Top of page
  2. Summary
  3. Introduction
  4. Results
  5. Discussion
  6. Experimental procedures
  7. Acknowledgements
  8. References
  9. Supporting Information

Protein secretion systems are critical to bacterial virulence and interactions with other organisms. The Type VI secretion system (T6SS) is found in many bacterial species and is used to target either eukaryotic cells or competitor bacteria. However, T6SS-secreted proteins have proven surprisingly elusive. Here, we identified two secreted substrates of the antibacterial T6SS from the opportunistic human pathogen, Serratia marcescens. Ssp1 and Ssp2, both encoded within the T6SS gene cluster, were confirmed as antibacterial toxins delivered by the T6SS. Four related proteins encoded around the Ssp proteins (‘Rap’ proteins) included two specifically conferring self-resistance (‘immunity’) against T6SS-dependent Ssp1 or Ssp2 toxicity. Biochemical characterization revealed specific, tight binding between cognate SspRap pairs, forming complexes of 2:2 stoichiometry. The atomic structures of two Rap proteins were solved, revealing a novel helical fold, dependent on a structural disulphide bond, a structural feature consistent with their functional localization. Homologues of the Serratia Ssp and Rap proteins are found encoded together within other T6SS gene clusters, thus they represent founder members of new families of T6SS-secreted and cognate immunity proteins. We suggest that Ssp proteins are the original substrates of the S. marcescens T6SS, before horizontal acquisition of other T6SS-secreted toxins. Molecular insight has been provided into how pathogens utilize antibacterial T6SSs to overcome competitors and succeed in polymicrobial niches.


Introduction

  1. Top of page
  2. Summary
  3. Introduction
  4. Results
  5. Discussion
  6. Experimental procedures
  7. Acknowledgements
  8. References
  9. Supporting Information

Protein secretion systems and their substrates are central to bacterial virulence and interaction with other organisms (Gerlach and Hensel, 2007). Six different secretion systems (Types I–VI) are used by Gram-negative bacteria to transport specific proteins to the exterior of the bacterial cell or further inject them into target cells. The most recently described of these is the Type VI secretion system (T6SS) (Filloux et al., 2008). T6SSs are complex multi-protein assemblies that span both bacterial membranes and inject effector proteins directly from the bacterial cytoplasm into target cells (Bonemann et al., 2010; Cascales and Cambillau, 2012). T6SSs are encoded by large, variable gene clusters that contain 13 ‘core’ essential components, believed to make up the basic secretion apparatus. Two core proteins, Hcp and VgrG, form the extracellular part of the secretion machinery and depend on a functional T6SS apparatus for their movement to the outside of the bacterial cell (indeed, the presence of Hcp in the secreted fraction has provided a useful assay for basic T6SS assembly and activity; Pukatzki et al., 2009). Hcp and VgrG most likely form a needle-like membrane-puncturing device related to the bacteriophage tail spike; this structure is believed to be pushed to the outside of the secreting cell and likely into target cells upon contraction of a tail sheath-like structure (Leiman et al., 2009; Bonemann et al., 2010; Basler et al., 2012). T6SSs occur in many pathogenic bacteria and are implicated in virulence in important pathogens, including Burkholderia mallei, Burkholderia pseudomallei, Burkholderia cenocepacia, Vibrio cholerae, Aeromonas hydrophila, Edwardsiella tarda and Pseudomonas aeruginosa (Zheng and Leung, 2007; Cascales, 2008; Jani and Cotter, 2010; de Pace et al., 2010; Burtnick et al., 2011; Rosales-Reyes et al., 2012). In several cases, the action of such ‘anti-eukaryotic’ T6SSs appears to result in disruption of the actin cytoskeleton (Pukatzki et al., 2007; Aubert et al., 2008; Suarez et al., 2010). Exciting recent work has demonstrated that some T6SSs are used to target other bacteria, efficiently killing or inhibiting competitors. This has been reported for T6SSs in P. aeruginosa, Burkholderia thailandensis, V. cholerae and Serratia marcescens (Hood et al., 2010; MacIntyre et al., 2010; Schwarz et al., 2010; Murdoch et al., 2011). The discovery that certain T6SSs may be ‘antibacterial’ rather than, or in addition to, ‘anti-eukaryotic’ is highly relevant to the competitive fitness and success of pathogens, particularly within polymicrobial infection sites. Such a system could provide the pathogen with a large competitive advantage against other bacteria in the host or the environment, enabling it to proliferate and mount a successful infection.

Identifying the proteins secreted by T6SSs is a priority, as they will be the ‘effectors’ that directly act on target eukaryotic or bacterial cells. A special case of T6-secreted effector is the class of ‘evolved’ VgrG proteins found in a minority of T6SSs which have extra C-terminal effector domains, e.g. the actin cross-linking domain of V. cholerae VgrG1 that is translocated into mammalian cells (Pukatzki et al., 2007; Jani and Cotter, 2010). However, excluding the structural components VgrG and Hcp, very few ‘true’ T6SS-secreted proteins have been confirmed so far. Best characterized are three effector proteins, antibacterial toxins named Tse1–3, secreted by the antibacterial HSI-1 T6SS of P. aeruginosa. Tse1 and 3 are peptidoglycan hydrolases that attack the cell wall of target bacteria (Hood et al., 2010; Russell et al., 2011). Tse2 is active in the cytoplasm of target cells, where it efficiently induces quiescence (Li et al., 2012). All three have adjacently encoded cognate ‘immunity’ proteins (Tsi1–Tsi3) which protect the secreting cell from harming itself or being harmed by its sibling neighbours (Hood et al., 2010; Russell et al., 2011). Significantly, obvious homologues of the Tse and Tsi proteins are not detectable outside of P. aeruginosa (Hood et al., 2010). A recent report has also identified a number of candidate T6SS substrates in B. thailandensis, one of which was confirmed as a new T6-secreted peptidoglycan amidase (Russell et al., 2012).

Opportunistic Gram-negative bacteria cause a large proportion of problematic and antibiotic-resistant hospital-acquired infections. Enterobacteria (especially extended-spectrum β-lactamase producing isolates) are among the leading culprits, including S. marcescens (Choi et al., 2007; Lockhart et al., 2007). We previously reported that S. marcescens Db10 possesses a T6SS with potent antibacterial activity (Murdoch et al., 2011). How this activity is mediated, in particular the antibacterial effectors secreted by the T6SS, was unknown. Hence, we sought to identify and characterize novel antibacterial effectors secreted by the S. marcescens T6SS. We report the identification and characterization of two such effectors, Ssp1 and Ssp2, which are encoded within the T6SS gene cluster and represent novel T6-secreted antibacterial toxins. We have also identified and characterized the Rap proteins, which include the cognate immunity proteins to these toxins. Biochemical analyses demonstrated a tight and specific interaction between secreted and immunity proteins. These secreted toxins and immunity proteins represent two new protein families, co-occurring within T6SS gene clusters of many other organisms. Additionally, determination of high-resolution crystal structures of two members of the Rap protein family revealed that this family possesses a previously undescribed protein fold that is dependent on formation of a disulphide bond.

Results

  1. Top of page
  2. Summary
  3. Introduction
  4. Results
  5. Discussion
  6. Experimental procedures
  7. Acknowledgements
  8. References
  9. Supporting Information

The T6SS gene cluster harbours self-resistance determinants and candidate secreted effectors

The T6SS gene cluster of S. marcescens Db10, SMA2244–2281, contains 38 genes, including many with no known function (Murdoch et al., 2011). We speculated that encoded within this cluster might be T6-secreted effectors and/or self-resistance determinants, the latter preventing the T6SS-expressing cell from harming itself or being harmed by its isogenic (sibling) neighbours. In order to determine whether the cluster did indeed contain self-resistance determinants (such as specific immunity proteins analogous to the Tsi proteins), we generated a mutant lacking the entire T6SS gene cluster (ΔT6SS) and examined whether it was fully resistant to the T6SS of the wild type strain. Co-culture of two target strains, wild type Db10 and the ΔT6SS mutant, each with a wild type and a ΔclpV attacker, showed that the ΔT6SS mutant had lost resistance to T6SS-mediated inhibition or killing by the wild type strain (Fig. 1A, left). Recovery of ΔT6SS was decreased 100-fold when it was co-cultured with the wild type strain, compared with when the wild type strain was co-cultured with itself. This effect was dependent on a functional T6SS in the attacker as there was no loss of ΔT6SS when it was co-cultured with a ΔclpV mutant. The ATPase ClpV is one of the core, structural components of the T6SS and we have shown previously that it is essential for Hcp secretion and T6-mediated antibacterial killing activity of S. marcescens Db10 (Murdoch et al., 2011). To simplify the analysis of multiple mutants, we defined the ‘resistance index’ of a strain as the difference between recovery when co-cultured with the wild type strain and recovery when co-cultured with the ΔclpV mutant, specifically log2[recovery vs. wild type/recovery vs. ΔclpV]. The wild type or other resistant strain will show no difference and have a resistance index of 0. A target strain with reduced ability to resist harm caused by the T6SS will have a negative resistance index, exemplified by the ΔT6SS mutant with a resistance index of −7.6 (Fig. 1A, right). Self-resistance did not depend on an active T6SS, as a ΔclpV mutant had a resistance index of 0. Similarly, mutants in other essential core T6SS components, Δlip, ΔicmH and ΔtssK (Murdoch et al., 2011) also showed no loss of self-resistance (data not shown). Therefore, genes other than those encoding the core conserved T6SS components were implicated in self-resistance. Our attention was particularly caught by a locus in the middle of the gene cluster, where six non-conserved genes, SMA2260–2262, SMA2264–2266, are flanked by conserved T6SS components. A mutant lacking all of these genes (but maintaining intact SMA2263, encoding Hcp1) was also tested and found to have a negative resistance index (Fig. 1A). Hence, one or more of these genes contributes to self-resistance and may encode immunity protein(s).

figure

Figure 1. An internal locus in the S. marcescens T6SS gene cluster encodes secreted proteins and self-resistance functions.

A. T6SS-mediated inhibition of self in the absence of genes within the T6SS gene cluster. Left: number of recovered target cells, either wild type (WT) or ΔT6SS mutant (ΔSMA2244–2281), following co-culture (1:1) with the attacking strain, WT or ΔclpV (T6SS inactive mutant). Right: resistance index, defined as log2[recovery of target in presence of wild type/recovery of target in presence of ΔclpV], of wild type Db10, ΔclpV, ΔT6SS or a mutant lacking genes SMA2260–2262 and SMA2264–2266. Bars show mean ± SEM (n = 4).

B. and C. Schematic depiction of loci containing genes encoding the Rap and Ssp genes in S. marcescens Db10 (B) and homologues in selected other organisms (C). Rap family proteins are shown in purple, Ssp family proteins in green, conserved T6SS core genes in grey, and Hcp homologues in dark grey. In (B) cellular localization and theoretical mass and pI of the proteins are given beneath the corresponding gene.

D. Secretion of Hcp1 by wild type and mutants of S. marcescens Db10 as shown by anti-Hcp1 immunoblotting of cellular and secreted fractions. Δrap1ab,ssp1 indicates a mutant lacking the rap1a, rap1b and ssp1 genes; Δrap2ab,ssp2 indicates a mutant lacking the rap2a, rap2b and ssp2 genes; Δssp1,ssp2 indicates a mutant lacking the ssp1 and ssp2 genes, and Δrap,ssp indicates a mutant lacking all of the rap and ssp genes.

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Closer examination of the proteins encoded by SMA2260–2262 and SMA2264–2266 revealed two classes of small proteins (Fig. 1B). SMA2261 and SMA2264 were basic proteins with detectable sequence similarity between them, no discernable cellular localization signals and no predicted function. We hypothesized that they might be secreted substrates, and, given subsequent results, named them Ssp1 and Ssp2 (Secreted small protein). SMA2260, SMA2262, SMA2265 and SMA2266 were proteins with classical Sec-dependent N-terminal signal peptides, identified using SignalP (Petersen et al., 2011), and thus predicted to be periplasmic. They also had no predicted function but shared detectable sequence similarity with each other. We hypothesized that they would represent specific immunity proteins or other self-resistance determinants, and named them Rap1a, Rap1b, Rap2a and Rap2b (Resistance associated protein). The genes encoding all these small proteins fall into two sets, either side of hcp1 and within genes encoding T6SS structural proteins, vipB and fha (Fig. 1B). Homologues of the Ssp and Rap proteins are encoded within T6SS gene clusters in many other bacterial species (and in at least one case apart from the T6SS) and appear to always co-occur (see representative examples in Fig. 1C). We speculated that the S. marcescens Ssp and Rap proteins represented previously unknown combinations of T6-secreted effectors and cognate immunity proteins. Importantly, mutants lacking one, some or all of the small proteins exhibited wild type levels of Hcp secretion (Figs 1D and S1). Thus, none of the Ssp or Rap proteins is required for Hcp secretion, i.e. they play no structural role in the T6SS.

Ssp1 and Ssp2 are Type VI-secreted effectors

Ssp1 and Ssp2 were shown to be secreted substrates of the T6SS by immunoblotting secreted fractions from the wild type strain, two T6SS mutants, ΔclpV and ΔtssE, and the corresponding complemented strains, using specific anti-Ssp1 and anti-Ssp2 antibodies. Both proteins were detected in the culture supernatant, entirely dependent on a functional T6SS (Fig. 2A). Neither protein was detectable in the cellular fraction, implying they were rapidly turned over if not secreted (data not shown). Secretion of Ssp2 was also independent of Ssp1, and vice versa, again confirming they have no structural or accessory role in the secretion machinery (Fig. 2A). In order to establish if the Ssp proteins were antibacterial toxins contributing to the killing or inhibition of the susceptible ΔT6SS mutant by the wild type strain, the recovery of ΔT6SS in the presence of different mutants was determined. Recovery of the ΔT6SS target was increased fivefold with the Δssp2 mutant, or any multiple mutant lacking ssp2, as attacker, compared with the wild type attacker (Fig. 2B). In contrast, in this assay, loss of Ssp1 did not cause a statistically significant impairment in killing of ΔT6SS. None of the Rap proteins was required for targeting of ΔT6SS (Fig. 2B).

figure

Figure 2. Proteins Ssp1 and Ssp2 are secreted by the Type VI secretion system and self-harm is mediated by Ssp2.

A. Immunoblot detection of Ssp1 and Ssp2 in the secreted fraction of the strains indicated using antibodies against Ssp1, Ssp2 or RNAP (lysis control); levels of RNAP in the cellular fraction are also shown. Strains are: wild type S. marcescens Db10 (WT); mutants Δssp1, Δssp2, ΔtssE, ΔclpV; mutants carrying vector control plasmids (+VC, pSUPROM) and mutants carrying complementing plasmids (ΔtssE + TssE, pSC045; ΔclpV + ClpV, pSC039).

B. Recovery of the ΔT6SS mutant as the target strain following co-culture with the different attacking strains indicated, expressed relative to recovery of ΔT6SS when co-cultured with wild type Db10. Bars show mean ± SEM (n ≥ 4); *** indicates a significant difference compared with the wild type strain (P < 0.001).

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Self-resistance against the Ssp1 and Ssp2 toxins is mediated by their cognate Rap partners

In order to assess the contribution of each of the rap (and ssp) genes to self-resistance, single mutants were constructed. It rapidly became apparent that single mutants in rap1a and rap2a had severe fitness defects on solid media, both on rich (Fig. 3A) and minimal media (Fig. S2), and particularly Δrap2a. Culture spots and single colonies of each mutant were ‘thinner’, smaller (in the case of Δrap2a), and with altered surface morphology. Examination of single cells showed that the Δrap1a cells appeared bigger and less uniformly shaped than wild type cells and the Δrap2a cells had striking phenotypes, being either markedly distended or highly elongated (Figs 3A and S2). These phenotypes could be complemented by expression of the corresponding gene in trans (indeed, the additional stress of the selective antibiotic made the phenotypes of Δrap1a and Δrap2a mutants carrying vector control plasmids even more pronounced; Fig. 3A). In contrast, when Δrap1a was constructed in combination with Δssp1, or Δrap2a in combination with Δssp2, the double mutants were readily made and were of normal appearance and fitness on solid media (Figs 3A and S2). These observations are entirely consistent with Rap2a serving as the immunity protein against the Ssp2 toxin and Rap1a being the cognate immunity protein alleviating toxicity mediated by Ssp1. Similarly, when Δrap1a or Δrap2a mutants were constructed in combination with the ΔclpV mutation, the double mutants were again apparently healthy on solid media (Figs 3A and S2). Hence, self-toxicity depended on a functional T6SS, implying it was caused by T6SS-mediated injection of the toxin into a susceptible cell by its neighbours (further supported by the observation that Δrap1a and Δrap2a did not display comparable growth defects in liquid culture, where contact-dependent targeting is unlikely to occur efficiently; Fig. S2).

figure

Figure 3. Self-resistance is mediated by specific Rap immunity proteins cognate to the secreted Ssp proteins.

A. Phenotypes of wild type S. marcescens Db10 (WT) and selected single and double mutants after growth on solid LB media for 24 h. For each strain, representative images of the morphology of a culture spot (left, scale bar 2 mm), single colonies (middle, scale bar 1 mm) and individual cells (right, scale bar 10 μm) are shown. Mutants carrying complementing plasmids are Δrap1a + Rap1a (pSC538) and Δrap2a + Rap2a (pSC542); the vector control plasmid (VC) was pSUPROM.

B. Resistance index of wild type Db10 and the deletion mutants indicated as target strains.

C. Recovery of a Δrap2a mutant (Δrap2aclpV) as the target strain following co-culture with the different attacking strains indicated, expressed relative to recovery of target when co-cultured with the ΔclpV mutant. All strains carry the vector control plasmid pSUPROM, except for Δssp2 + Ssp2, in which the mutant carries the complementing plasmid pSC541. In (B) and (C), bars show mean ± SEM (n ≥ 4); *** indicates a significant difference compared with the wild type strain (P < 0.001).

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An immunity function for Rap2a was directly demonstrated in co-culture (antibacterial competition assay): target strains containing a Δrap2a mutation all showed a negative resistance index (Fig. 3B; the single Δrap2a mutant was not tested because of its severe sickness). Strains containing a Δrap1a mutation did not have a negative resistance index, consistent with the lack of significant contribution of Ssp1 to self-killing under the conditions of these assays (Fig. 2B). To confirm that Ssp2 was directly and entirely responsible for the inhibitory effect of a wild type attacker strain on Δrap2a, we showed that a Δrap2a target strain is completely resistant to attack by a Δssp2 mutant, with recovery of Δrap2a in the presence of a Δssp2 attacker being the same as its recovery in the presence of a ΔclpV attacker (Fig. 3C). Additionally, inhibition of Δrap2a target was restored to wild type levels when the Δssp2 mutant attacker was complemented by expression of Ssp2 in trans. The susceptibility of Δrap2a to killing by the wild type strain could also be fully complemented (Fig. S2). Hence, Ssp2 and Rap2a represent a specific, cognate toxin and immunity protein pair.

Biochemical studies confirm a strong interaction between cognate secreted toxins and immunity proteins

Each of the Ssp and Rap proteins was overproduced and purified (in the case of the Rap proteins, without their N-terminal signal peptides). Complex formation was demonstrated using size exclusion chromatography (SEC) analysis. All Rap proteins were dimeric in solution, whereas Ssp1 and Ssp2 were monomeric (Fig. 4A and B). When equimolar amounts of Ssp1 and Rap1a were mixed, all of the protein was detected in a higher molecular weight complex (Fig. 4A) and the same was also observed on mixing Ssp2 and Rap2a (Fig. 4A). In contrast, no complex formation between Ssp1 and Rap1b or between Ssp2 and Rap2b, no additional three-way complexes and no ‘cross’ interactions between Ssp2 and Rap1a or between Ssp1 and Rap2a were observed (Figs 4B and S3). As mixing equimolar amounts of Ssp1 and Rap1a resulted in detection of only the complexed species, with no unbound form of either protein detectable, this implied a 1:1 molar complex. The 1:1 molar stoichiometry of the Rap1a–Ssp1 complex was confirmed by quantitative analysis of the composition of the higher molecular weight peak using in-gel SYPRO Orange staining (Rickman et al., 2004) (Fig. 4C). Given the dimeric nature of Rap1a and an apparent complex mass by SEC of around 55 kDa [predicted Mw of 1:1 molar complexes are 34.6 kDa (1:1), 69.2 kDa (2:2), 104 kDa (3:3) or 138 kDa (4:4)], this is most consistent with a heterotetrameric Rap1a2–Ssp12 complex. Similar logic supported a Rap2a2–Ssp22 complex (Fig. 4A and C). The SEC analyses suggested stable complexes were formed between the cognate Ssp and Rap proteins. Isothermal titration calorimetry (ITC) analysis of complex formation between Ssp1 and the Rap1a dimer and between Ssp2 and the Rap2a dimer (Fig. 4D) showed that, in both cases, binding was clearly exothermic and tight, at least in the low nanomolar Kd range. Although apparent Kd values of 4–8 nM were obtained, this is approaching the limit of accuracy for conventional ITC (Wiseman et al., 1989). Finally, we took advantage of the tight Rap–Ssp interactions to utilize immobilized Rap2a and Rap1a to affinity-purify secreted Ssp2 or Ssp1, respectively, from culture supernatant (Figs 4E and S3). Mass spectrometry not only confirmed the identity of Ssp1 and Ssp2 but also showed that Ssp2 is not processed on secretion, as almost complete sequence coverage revealed intact N- and C-termini (Fig. S3). For Ssp1, we observed an intact C-terminus but the sequence of the very N-terminus corresponds to several tryptic peptides too small to be detectable by standard mass spectrometry, so we were unable to definitively confirm lack of processing at this end (data not shown).

figure

Figure 4. In vitro interaction between cognate secreted toxins and immunity proteins.

A. and B. SEC analysis of complex formation between the proteins indicated. Ten nanomoles of the protein (or of each protein in the case of mixtures) was separated on a calibrated Superdex 75 10/300 GL column. The theoretical molecular mass of each monomer is given.

C. In-gel SYPRO Orange staining and quantification of the relative molar amounts of Rap1a and Ssp1 (left) or Rap2b and Ssp2 (right) in samples from the complex-containing peaks observed in SEC (A).

D. ITC analysis of the interaction between Ssp1 and Rap1a (left) and Ssp2 and Rap2a (right).

E. Affinity isolation of secreted Ssp2 from culture supernatant using immobilized immunity protein His-Rap2a as bait. Supernatant samples (Supt) were prepared from the strains indicated (WT, wild type). The band indicated by arrowhead was identified as Ssp2 by mass spectrometry.

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The secreted small proteins, Ssp1 and Ssp2, exert distinct harmful effects when targeted to the periplasm in Escherichia coli and are neutralized by coexpression of the cognate immunity protein

In order to confirm the antibacterial toxin function of Ssp1 and Ssp2 and establish in which cellular compartment they exerted their effect, each protein was produced in E. coli, either in the cytoplasm or artificially targeted to the periplasm (by the N-terminal fusion of the Sec-dependent OmpA signal peptide: sp-Ssp2 or sp-Ssp1). The presence of Ssp2 in the periplasm, but not the cytoplasm, prevented growth of E. coli on LB and minimal media; this toxicity was alleviated by the co-production of Rap2ab (Fig. 5A). Periplasmic Ssp1 was also toxic and its effect alleviated by co-production of Rap1ab (Fig. 5A). However Ssp1 toxicity was only observed at higher expression levels and on minimal media. The periplasmic localization of the Rap proteins in S. marcescens was confirmed by fractionation and immunoblotting of epitope-tagged versions of the protein (Fig. 5B, data not shown).

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Figure 5. Differential periplasmic toxicity of Ssp1 and Ssp2 and periplasmic localization of Rap proteins.

A. Growth of E. coli MG1655 transformed with (i) plasmids expressing Ssp2 (pSC133), Ssp2 + Rap2a + Rap2b (pSC134), OmpAsp-Ssp2 (pSC138) or OmpAsp-Ssp2 + Rap2a + Rap2b (pSC144) from an arabinose-inducible promoter, or with the empty vector (vector, pBAD18-Kn), on LB or M9 media containing 0.2% glucose, 0.02% arabinose or 0.2% arabinose; or (ii) the equivalent analysis using plasmids expressing Ssp1 (pSC151), Ssp1 + Rap1a + Rap1b (pSC159), OmpAsp-Ssp1 (pSC152) or OmpAsp-Ssp1 + Rap1a + Rap1b (pSC160).

B. Localization of RNAP (RNA polymerase, cytoplasmic marker protein), MBP (maltose binding protein, periplasmic marker protein) and HA-tagged Rap proteins. Wild type S. marcescens Db10 expressing Rap1a-HA (pSC538), Rap2b (pSC543) or the vector control (pSUPROM) was subjected to fractionation (WC, whole cell; PP, periplasm; CM, cytosol + membranes), followed by immunoblotting with anti-RNAP, anti-MBP or anti-HA antibodies as indicated.

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Next, we also determined whether Ssp2 and/or Ssp1 were essential for the observed antibacterial activity of the S. marcescens T6SS against other bacterial species (Murdoch et al., 2011). Neither protein was required for T6SS-dependent killing of other bacteria (Fig. S4). This implies redundancy of effector function, in other words that other T6SS-secreted toxins are still able to cause killing in the absence of Ssp1 and Ssp2.

The Rap family of proteins display a new fold

Bioinformatic analysis of the Rap protein sequences predicted similarities between them, despite relatively low sequence conservation, e.g. mature Rap1b and Rap2b share around 20% identity, as do mature Rap2a and Rap2b. All four Rap proteins appeared to be highly acidic, to carry an N-terminal periplasmic targeting signal sequence of about 24 residues, and were predicted to have similar α-helical structures (using PSIPRED). In addition, a cysteine pairing appeared to be conserved. Intriguingly, no structural relative of the Rap proteins could be identified; hence, we sought to obtain three-dimensional models using single crystal X-ray diffraction. Soluble recombinant Rap proteins were only obtained in high yield from E. coli Rosetta-gami (DE3), a strain engineered to support disulphide bond formation, and were dimeric in solution (Fig. 4). Well-ordered crystals of Rap1b and Rap2b were obtained and the structures were elucidated at 1.9 Å and 2.0 Å resolution respectively (Fig. 6, Table 1). A search for structural relatives using PDBeFold (pdbe.org/fold) and ProFunc (Laskowski et al., 2005) was performed using monomers and dimers of Rap1b and Rap2b as templates. The only matches were to short segments of α-helices with Z-scores (< 3) indicating low statistical significance. The lack of any convincing structural relationships indicates that the fold observed in both Rap1b and Rap2b is previously uncharacterized.

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Figure 6. Structural features of Rap1b and Rap2b dimers. The dimers are oriented to provide a view down their twofold axis of symmetry.

A. Ribbon diagram with helices of one Rap1b subunit coloured green, and the symmetry related molecule bronze. Elements of secondary structure, the N- and C-terminal residues are labelled and I ions are depicted as orange spheres. The disulphide bond is shown as yellow sticks and labelled.

B. Ribbon diagram of Rap2b with helices of one subunit blue, and the partner cyan.

C. and D. Electrostatic surface representation of Rap1b and Rap2b dimers in the same orientation as in (A) and (B). The electrostatic charge is contoured at 1 kT/e and −1 kT/e; negative (acidic) charge is red, positive (basic) blue. Residues that contribute to the basic patches are identified.

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Table 1. Crystallographic statistics for the Rap1b and Rap2b structures
 Rap1bRap2b
  1. a

    Values in parentheses refer to the highest resolution shell.

  2. b

    Rmerge = ΣhklΣi|Ii(hkl) − < I(hkl) > |/ΣhklΣi Ii(hkl), where Ii(hkl) is the intensity of the ith measurement of reflection hkl and <I(hkl)> is the mean value of Ii(hkl) for all i measurements.

  3. c

    Rwork = Σhkl||Fo| − |Fc||/Σ|Fo|, where Fo is the observed structure factor and Fc is the calculated structure factor.

  4. d

    Rfree is the same as Rcryst except calculated with a subset, 5%, of data that are excluded from the refinement calculations.

  5. e

    Diffraction Precision Index (Cruickshank, 1999).

  6. The PDB accession codes are 4AX2 (Rap1b) and 4B6I (Rap2b).

Space groupP3121P2221
a, b, c (Å)77.9, 77.9, 50.648.1, 57.0, 122.4
Resolutiona (Å)67.5–1.88 (1.98–1.88)44.78–2.0 (2.1–2.0)
No. reflections recorded162 739 (21 729)271 849 (36 384)
Unique reflections14 813 (2130)23 666 (3390)
Completeness (%)100.0100.0
Multiplicity/<I/σI>11.0 (10.2)/26.6 (5.9)11.5 (10.7)/25.7 (10.0)
Anomalous completeness (%)100.0100.0
Anomalous redundancy5.6 (5.1)6.0 (5.5)
Wilson B2)28.320.6
Residues/waters/ligands119/117/7392/137/–
Rmergeb (%)5.3 (38.3)8.5 (35.0)
Rworkc, Rfreed (%)18.3/22.118.9/24.8
Ave. B-factor (Å2)  
Chain A, B, C, D21.110.6, 9.8, 7.8, 8.9
Waters, iodides, ethylene glycol42.3, 49.4, 55.714.6
Cruickshank DPIe (Å)0.10.2
Ramachandran plot  
Most favoured118 residues381
Additional allowed110
Outliers0Gln74
R.m.s.d. on ideal values  
Bond lengths (Å) angles (°)0.02/1.510.02/1.79

The asymmetric unit of the Rap1b structure consists of a single subunit and crystallographic symmetry generates the dimer. Rap2b has two dimers, formed by subunits A : B and C : D, in the asymmetric unit. The four subunits are similar, with the root-mean-square deviation (r.m.s.d.) between superimposed Cα atoms ranging from 0.5 Å (subunit B and D) to 0.7 Å (subunits A and C). The two proteins display obvious similarities in terms of secondary, tertiary and quaternary structure (Figs 6 and S5). An overlay of Rap1b and Rap2b subunits matches 71 Cα atoms with a r.m.s.d. of 1.4 Å. Of note is the conservation of the disulphide bond, a key structural feature, likely critical to the stable folding of the subunit and subsequent dimerization of the Rap proteins. The Rap subunit is constructed around a helical bundle of five helices (α2–α6). A disulphide linkage (Cys54–Cys120 in Rap1b, Cys41–Cys101 in Rap2b) tethers α2 and α5 together. This association in turn supports formation of a hydrophobic core that is primarily aliphatic with residues contributed from α2, α4, α5 and α6. Three helices (α2, α3, α5) form a concave surface on one side of the monomer. A series of hydrogen bonding interactions also helps to stabilize the arrangement of α2 and α4. By virtue of being longer than Rap2b, Rap1b has an extension of five residues at the N-terminus and 13 at the C-terminus, the latter of which form a short helix α7. These segments of Rap1b are on the surface of the molecules at opposite ends of the dimer (Fig. 6).

The Rap proteins display an extensive dimerization interface (Fig. 6), consistent with the observation that each Rap protein exists as a stable dimer in solution (Fig. 4A and B). The Rap1b dimer uses almost 24% of the accessible surface area of a subunit in formation of the dimer. In the case of Rap2b the value is 20%. Such percentages are indicative of highly stable oligomers (Krissinel and Henrick, 2007). The dimer is stabilized by extensive van der Vaals interactions primarily involving aliphatic residues, in conjunction with hydrogen bonding interactions and solvent mediated bridging associations. The most important contributions are from side-chains on the concave surface, formed by α2, α3 and α5, interacting with the partner across the molecular twofold axis of symmetry. Additional interactions involve a self-association of the loop that links α2 and α3, together with the N-terminus α1 and α5. Helices α2 and α5 are thus not only critical for the fold of the Rap subunits but also to creating a suitable interface that leads to a highly stable dimer. This observation, together with the conserved disulphide bond (Fig. 7), ties in with the localization of Rap proteins to the oxidative environment of the periplasm where correct folding to support anti-toxin activity must occur.

figure

Figure 7. Conservation of the Rap protein fold. Sequence alignment of S. marcescens Rap2b and Rap2a with homologous proteins from Erwinia amylovora (GenBank CBA22869.1), Enterobacter cloacae (NCBI Reference Sequence YP_003612051.1), Cronobacter sakazakii (NCBI Reference Sequence YP_001439955.1), Salmonella Typhimurium (NCBI Reference Sequence NP_459276.1) and Pseudomonas syringae (NCBI Reference Sequence YP_237109.1). The secondary structure of Rap2b (blue cylinders) and the predicted secondary structure of the P. syringae protein (purple cylinders) are shown. All proteins had similar predicted secondary structures (PSIPRED); the one shown is representative. Cysteine residues involved in disulphide bond formation are coloured yellow. Alignment was generated using T-Coffee and annotated using ALINE, using the mature proteins (i.e. without N-terminal signal peptides; numbering refers to the full-length proteins).

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Importantly, sequence analysis and secondary structure predictions for the other Rap proteins, in S. marcescens and other organisms, suggest strongly that the novel fold revealed by our crystallographic analyses is generic for this entire family of proteins (Fig. 7). Not only are the main α-helices observed in both crystal structures closely mimicked by the structural predictions of the other members of the family, the Cys residues contributing to the structural disulphide bond are also conserved. Additionally, Rap2b shares slightly higher sequence identity with Rap2a (23% identity for the mature proteins) than it does with Rap1b (20% identity). Given the similarity of the Rap1b and 2b crystal structures, discussed above (Fig. S5), then this provides confidence that Rap2a shares this new fold and indeed that the Rap fold is a defining characteristic of this protein family, many members of which are likely to represent T6SS immunity proteins.

Discussion

  1. Top of page
  2. Summary
  3. Introduction
  4. Results
  5. Discussion
  6. Experimental procedures
  7. Acknowledgements
  8. References
  9. Supporting Information

In this study we have identified two proteins, Ssp1 and Ssp2, as true (non-structural) secreted substrates of the S. marcescens T6SS and confirmed them as new T6SS-dependent antibacterial toxins. We have also demonstrated, genetically and biochemically, that the highly specific, cognate periplasmic immunity proteins, Rap1a and Rap2a, efficiently neutralize the effect of the Ssp proteins. The atomic structures of two other, related Rap proteins reveal that the immunity proteins should exhibit a novel protein fold likely only attained when they are present in the periplasm.

Our examination of Ssp1 and Ssp2 suggested that they represented novel antibacterial toxins, containing a domain of unknown function, DUF4285, present in prokaryotic and eukaryotic proteins. We were unable to detect significant sequence similarity with well-known peptidoglycan hydrolases and the structure prediction program Phyre2 (Kelley and Sternberg, 2009) was unable to assign them any peptidoglycan hydrolase-like structure. Nevertheless, as they are clearly periplasmic-acting toxins (Fig. 5) and non-resistant mutants showed apparent lytic and/or division defects (Figs 3A and S2), a cell wall targeting function seemed most likely. This idea has very recently been strongly supported by the observation that related proteins exhibit peptidoglycan amidase activity in vitro (see below; Russell et al., 2012). Importantly, through analysing secreted Ssp2 isolated from culture supernatant, we have also shown for the first time that T6-secreted effectors are not processed at either terminus during secretion. It seems clear that Ssp1 and Ssp2 are not the only effector proteins secreted by the S. marcescens T6SS. First, Ssp mutants are still able to kill Pseudomonas fluorescens as effectively as wild type Db10 (Fig. S4), implying that other toxins secreted in their absence are sufficient to maintain efficient antibacterial killing. Additionally, the susceptibility of the ΔT6SS mutant to self-targeting by the wild type strain is greater than that of the Δrap,ssp mutant (Fig. 1A), implying additional immunity proteins and thus cognate secreted toxins within the T6SS gene cluster. Moreover, the magnitude of killing of the ΔT6SS mutant by wild type Db10 is less than that observed during T6-dependent killing of other organisms (Murdoch et al., 2011; Fig. S4), suggesting that additional secreted toxins (and cognate immunity proteins) are encoded elsewhere in the genome. Indeed, our unpublished work has identified four other, unrelated, candidate substrates of the Serratia T6SS. Hence, we believe that S. marcescens uses a species-specific arsenal of secreted toxins to produce the potent and efficient targeting of a variety of competitor bacteria observed (Murdoch et al., 2011).

Our work provides strong functional evidence for a new family of related T6SS substrates (Ssp1 and Ssp2 homologues) and family of related immunity proteins (Rap homologues) found in many different bacterial species and generally encoded within a main T6SS gene cluster of that organism. Ssp- and Rap-like proteins are found associated with a subset of T6SSs (some, but not all, closely related to the S. marcescens T6SS), but whether these T6SSs all exhibit antibacterial activity remains to be determined. While this report was in preparation, a bioinformatic study identified four disparate families of predicted T6-secreted peptidoglycan amidases, with Tse1 of P. aeruginosa being a member of ‘Family 1’ (Russell et al., 2012). Entirely consistent with our data, Ssp-like proteins were recognized as one of these families, ‘Family 4’. A related family of proposed cognate immunity proteins identified as co-occurring with all Ssp/Family 4 proteins is of course the Rap family proteins. Thus, in the nomenclature proposed by Russell et al., Ssp1 and Ssp2 could be classified as Tae4.1SM and Tae4.2SM, and Rap1a and Rap2a as Tai4.1aSM and Tai4.2aSM. Unlike Families 1–3, the Family 4/Ssp proteins are almost unrecognizable as peptidoglycan amidases at a sequence and structure prediction level. Nevertheless, the purified Ssp homologue STM0277 from Salmonella enterica serovar Typhimurium was able to hydrolyse peptidoglycan cross-links at the D-Glu-mDAP bond of the acceptor stem (Russell et al., 2012). Additionally, artificial expression and targeting of STM0277 to the periplasm was shown to be toxic to E. coli, with rescue by coexpression of the Rap homologue STM0278. However, studies were not conducted to show that STM0277 is a T6SS substrate or that it plays a role in T6-mediated antibacterial activity, neither was a role for STM0278 in self-resistance in the native, T6-elaborating organism investigated. In contrast, we have provided the comprehensive genetic, in vivo and biochemical data necessary to confirm that Ssp/Family 4 proteins are indeed a novel family of T6-secreted antibacterial toxins and moreover that the Rap family contains the cognate immunity proteins. Interestingly, it was recently reported that a mutant in the above Rap2a homologue in S. Typhimurium, STM0278, had a defect in replication in macrophages (Mulder et al., 2012). The reason behind this is not clear, but it may reflect the fact that this mutant has reduced fitness due to self-toxicity, just as we have shown for the Δrap2a mutant. It should also be noted that Ssp–Rap pairs are not always found associated with T6SS genes. A particularly interesting example is the location of such a pair almost adjacent to genes encoding a classical RelE–RelB toxin–antitoxin pair (T-AT; Yamaguchi and Inouye, 2011) on a plasmid in Acinetobacter baumannii (Fig. 1). It is tempting to speculate that an original source of T6 toxin/resistance pairs is from plasmid T-AT systems.

The work of Russell et al. (2012) combined with our demonstration that Ssp1 and Ssp2 function as periplasmic-acting toxins is highly consistent with these proteins having a peptidoglycan amidase enzymatic activity. Of particular note, conserved Cys and His residues predicted by Russell et al. to represent the catalytic amino acids mediating peptidoglycan amide bond hydrolysis can be readily identified in Ssp1 and Ssp2. These are Cys50 (NTCAVRMS) and His133 (GHIDLIEP) in Ssp1, and Cys50 (NACAIRMS) and His131 in Ssp2 (GHATLWNG), with the equivalent, conserved regions in STM0277 being (NACPIRMS and GHVTLWNG). However, crucially, our data on the Ssp and Rap proteins in the context of T6SS-mediated attack and defence in vivo reveal that the situation is more subtle than this. In particular, Ssp1 and Ssp2 are clearly not redundant, despite having the same postulated enzymatic function. Rather, they have distinct activities or roles, with Ssp2 apparently more potent. In particular, we noted that the Ssp-dependent morphological phenotypes of the Δrap1a and Δrap2a mutants are different (Figs 3A and S2), that toxicity in the E. coli periplasm is only medium-dependent for Ssp1 (Fig. 5), and that the two may be relevant in different biological contexts (e.g. Ssp1 does not significantly contribute to self-targeting under the conditions of our standard assay, yet is clearly required for the self-toxicity observed in a Δrap1a mutant). This specialization is consistent with a clear specificity for only the cognate Ssp–Rap partner, as we observed. In the native context, it is clear that none of the other three Rap proteins can confer cross-resistance to Ssp2 in the absence of Rap2a (nor did Ssp2 interact with Rap1a biochemically). The molecular basis for the difference between Ssp1 and Ssp2, which share 24% sequence identity, is not yet clear and will require further study, including determination of in vitro enzymatic activity and atomic structures.

The S. marcescens Rap proteins represent founder members of a new bacterial protein family, members of which represent immunity proteins for T6-secreted toxins, as exemplified by Rap1a and Rap2a. We have determined the structures of two members of this family, Rap1b and Rap2b, revealing a new protein fold. Given the sequence homology, conservation of key residues and shared predicted secondary structure throughout all members of the family (Fig. 7; Russell et al., 2012), this fold appears to be shared across members from different organisms. A conserved disulphide bond and the observed stable dimerization interface, together with canonical N-terminal signal sequences, are consistent with a periplasmic localization for all Rap family proteins. To date, the structures of two other T6 immunity proteins have been solved. The first is the cytoplasmic Tsi2 protein (Li et al., 2012; Zou et al., 2012). Like the Rap proteins, Tsi2 exhibits a helical fold, is acidic and exists as a stable dimer in solution. However, the structures of Tsi2 and the Rap proteins are unrelated. Second, and very recent, is the structure of the periplasmic Tsi1 protein, complexed with the secreted peptidoglycan hydrolase effector, Tse1 (Ding et al., 2012). Tse1 possesses a strikingly accessible active site, facilitating its promiscuous and toxic peptidoglycan amidase activity (Chou et al., 2012). Tsi1 binds to Tse1 in a 1:1 complex, occluding the substrate-binding site of Tse1 in order to neutralize its activity (Ding et al., 2012). Critically, although the Rap1a/Rap2a proteins and Tsi1 both mediate resistance to peptidoglycan hydrolase toxins, their structures now appear to be entirely unrelated. Tsi1 exhibits an all β fold, related to a classical β-propeller, whereas Rap family proteins exhibit a novel helical fold. This indicates that the mechanisms by which immunity proteins confer resistance may be divergent even among those with effectors of similar function. Rap1a and Rap2a have an obvious immunity phenotype specific to their cognate secreted toxins, Ssp1 and Ssp2. However, the role of Rap1b and Rap2b is not yet known. While they do not appear to play a role in self-resistance, they may play a role in resistance towards closely related bacteria secreting similar toxins. It is worth noting that other organisms also possess multiple Rap family proteins for a given Ssp family protein (Fig. 1C and data not shown); therefore, whatever the function of Rap1b and 2b turns out to be, it may not be unique to Serratia.

Complementing our genetic and phenotypic demonstration of the cognate toxin-immunity function of Ssp1–Rap1a and Ssp2–Rap2a, we report detailed biochemical characterization of the interactions between these purified T6-secreted toxins and immunity proteins. For efficient self-protection, these interactions should be tight and highly specific, as was observed. Formation of Ssp1–Rap1a and Ssp2–Rap2a complexes is exothermic, with low nanomolar Kd, and with a stoichiometry of 2:2. A binding affinity of this order agrees well with the Kd of 3 nM reported for the Tsi1–Tse1 interaction (Ding et al., 2012); however, the Tsi1–Tse1 complex has a stoichiometry of 1:1, again highlighting significant differences between different pairs of toxin-immunity proteins. The structure of a Ssp–Rap complex and arrangement of the subunits has yet to be determined, although it is likely that the two Ssp proteins bind to the same part of each Rap monomer, exploiting the twofold symmetry. Li et al. suggest that Tse2 interacts with an acidic patch on Tsi2 distal to the dimer interface (Li et al., 2012). They also note that, like many toxin–antitoxin pairs, the resistance proteins Tsi1–3 are more acidic than the toxin proteins Tse1–3. This pattern is strikingly followed with the Ssp (theoretical pI 9) and Rap (theoretical pI 5–6) proteins. Nevertheless, while the highly acidic Rap proteins bind their cognate Ssp partners, which are noticeably basic, with high affinity, the story is not as simple as charge complementarity. Surprisingly for proteins with such low pI values, the striking surface feature conserved in Rap1b and Rap2b structures is a crescent-shaped basic patch on either side of the dimer (Fig. 6C and D). It is possible that such a basic crescent, if present on toxin-binding Rap proteins, may contribute to orientation of the partner during binding; conversely, it might contribute to the lack of Ssp binding by Rap1b and Rap2b. Additionally, all four S. marcescens Rap proteins are acidic and both Ssp proteins basic, yet only two, highly specific interactions are observed (Rap1a–Ssp1 and Rap2a–Ssp2). While charge complementarity would be expected to be important for specific complex formation, it is likely that shape considerations play an equally important role. The structure of a toxin-immunity protein complex will be necessary to delineate the molecular features that govern specific Rap–Ssp association. We are working towards that goal.

In summary, our data support a model (Fig. 8) whereby Ssp1 and Ssp2 are toxins secreted by the S. marcescens T6SS into the periplasm of a neighbouring cell. If this is an isogenic sibling, the cognate Rap proteins provide an efficient protective barrier, effectively binding and sequestering the toxin, whereas if it is a competitor, Ssp1/2 are free to attack the cell wall. However, Ssp1 and Ssp2 are only two of multiple distinct T6-secreted toxins. This provides the observed redundancy of function: if Ssp1/2 are missing, the other toxins still cause the efficient death of a competitor. This ‘belt and braces’ approach provides great robustness: if a competitor becomes resistant to one or two toxins, the others will still provide the ability to kill or inhibit the competitor efficiently. Of course, the toxic effect of Ssp1/2 can be seen against self (if the cognate Rap is missing) as Db10 has resistance proteins to neutralize the other toxins. We believe that other effectors most likely act on different cellular targets, analogous to the Pseudomonas-specific, cytoplasmic-acting toxin, Tse2 (Li et al., 2012). Finally, we speculate that as the Ssp and Rap proteins are encoded within the T6SS gene cluster, and related genes are found associated with other T6SSs, particularly closely related ones, they may represent the ancestral substrates of the S. marcescens T6SS. Subsequently, other toxins could have been horizontally acquired from diverse sources and adopted by this highly versatile secretion machine. The exciting task of deciphering how such species- and strain-specific arsenals of toxins and immunity proteins are co-ordinated by the producing cell and how they contribute to the dynamic composition of polymicrobial communities in infection and the environment lies ahead.

figure

Figure 8. Model for action and context of Ssp and Rap proteins.

A. Wild type S. marcescens Db10 uses its T6SS to inject multiple different antibacterial toxins (solid circles), including Ssp2 (green), into a susceptible target competitor cell, cumulatively causing a rapid death. Ssp2 attacks the cell wall in the periplasm (peri); other toxins are likely to attack targets in the cytoplasm (cyto).

B. Another wild type cell is resistant to T6SS attack by its neighbour because of the presence of cognate immunity proteins for all the toxins (open circles). Rap2a dimers (purple) form a protective barrier in the periplasm, rapidly binding and sequestering Ssp2.

C. When a Δrap2a mutant of Db10 is the target strain, all of the effectors except for Ssp2 are still neutralized, but Ssp2 secreted by wild type cells is now able to cause toxicity in the target.

D. In a putative ancestral cell, T6SS secretion of Ssp2, but not other toxins later acquired by horizontal transfer, inhibits a competitor target cell. In this case, loss of Ssp2 (or resistance to Ssp2 in the target) would prevent inhibition.

For clarity, Ssp1 and Rap1a are not shown but would behave similarly to Ssp2 and Rap2a.

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Experimental procedures

  1. Top of page
  2. Summary
  3. Introduction
  4. Results
  5. Discussion
  6. Experimental procedures
  7. Acknowledgements
  8. References
  9. Supporting Information

Bacterial strains, plasmids and culture conditions

All strains and plasmids used in this study are detailed in Table S1. All mutants constructed in S. marcescens Db10 were in-frame deletion mutants, generated by allelic exchange as described previously (Murdoch et al., 2011). Streptomycin-resistant derivatives were generated by phage ϕIF3-mediated transduction of the resistance allele from S. marcescens Db11 (Petty et al., 2006). Plasmids for constitutive expression of proteins in S. marcescens were derived from pSUPROM, plasmids for arabinose-inducible protein expression were derived from pBAD18-Kn, and derivatives of the pET15b-TEV plasmid were generated for protein overexpression and purification. S. marcescens was grown at 30°C in LB (10 g l−1 tryptone, 5 g l−1 yeast extract, 10 g l−1 NaCl, with 1.5 g l−1 agar for solid media) or minimal media (40 mM K2HPO4, 15 mM KH2PO4, 0.1% (NH4)2SO4, 0.4 mM MgSO4, 0.2% glucose) and E. coli was normally grown at 37°C in LB or M9 minimal media (M9). M9 (Sambrook and Russell, 2001) contained 0.5% glycerol (plus stated concentrations of arabinose and glucose as required). Growth analyses were performed in 96-well plates in a BioTek Synergy platereader. When required, media were supplemented with antibiotics: ampicillin (Ap) 100 μg ml−1, kanamycin (Kn) 100 μg ml−1, streptomycin (Sm) 100 μg ml−1, chloramphenicol (Cm) 25 μg ml−1; to maintain repression of proteins expressed from pBAD18-Kn, 0.5% glucose was added to the media for cloning and maintenance.

Antibacterial competition/co-culture assays

These were based on the assay described previously (Murdoch et al., 2011). In brief, the attacker strain and target strain (both at OD600 0.5) were mixed at an initial ratio of 1:1 attacker : target, co-cultured on solid LB for 7.5 h at 30°C and then the surviving target cells enumerated by serial dilution and viable counts on streptomycin-containing media. The target strain was always the streptomycin-resistant version of the mutant in question (Table S1). Statistical significance testing was performed by ANOVA followed by Dunnett's post test (GraphPad Prism software).

Bioinformatic identification of homologues of Rap and Ssp proteins and determination of their genetic contexts utilized the blast servers and sequence databases at the NCBI (http://www.ncbi.nlm.nih.gov).

Immunodetection of secreted proteins

Anti-Hcp immunoblots were performed as described (Murdoch et al., 2011). For detection of Ssp1 and Ssp2, cellular and secreted fractions were prepared from 25 ml of culture grown for 7 h in LB. Secreted proteins were precipitated using 50:50 chloroform : methanol followed by methanol wash and resuspension in 2× gel sample buffer (Murdoch et al., 2011). Cellular samples were prepared by sonicating harvested cells in 20 mM Tris·HCl pH 7.5, 150 mM NaCl, 1 mM EDTA, 0.5% Triton X-100 and isolating the soluble fraction by centrifugation. Anti-Ssp1 and anti-Ssp2 rabbit polyclonal antibodies were raised to the purified proteins (Eurogentec, Belgium) and used at 1:1000; peroxidase-conjugated secondary (Thermo Fisher Scientific) was used at 1:10 000. Anti-RNAP β (Neoclone, USA) was used at 1:20 000, with anti-mouse secondary (Roche) at 1:10 000. In all cases, protein from the same number of cells was loaded in the secreted versus the cellular samples.

Localization of Rap-HA proteins

Fractionation was performed using a cold osmotic shock procedure. Following growth of cultures for 5 h in LB, Tris·HCl pH 7.8 was added to 5 ml of cells to a final concentration of 50 mM and the cells were incubated for 10 min at room temperature, then recovered by centrifugation and washed once in LB. Cell pellets were resuspended in 1 ml of 40% sucrose, 30 mM Tris·HCl pH 7.8, 2 mM EDTA and incubated for 10 min at 30°C. One hundred microlitres of this fraction (‘whole cell’) was removed for analysis. Remaining cells were recovered by centrifugation, resuspended in 900 μl of ice-cold water and incubated on ice for 10 min, resulting in the release of the periplasm. After centrifugation, 100 μl of the supernatant (‘periplasm’ fraction) was retained for analysis. The pellet, containing the ‘cytoplasm + membranes’ fraction, was resuspended in 900 μl of 50 mM Tris·HCl pH 7.8 and 100 μl retained for analysis. Equivalent amounts, on a per cell basis, of each fraction in each strain were assayed. Anti-RNAP β was used as above, anti-MBP (NEB) was used at 1:10 000 and anti-HA (Roche) was used at 1:6000, all with anti-mouse secondary as above.

Microscopic analysis of colony and cell morphology

Overnight cultures were normalized to OD600 0.5, diluted 10−2 (culture spots) or to obtain single colonies, 10 μl spotted onto solid media and grown for 24 or 48 h. Macroscopic morphology of culture spots and single colonies were recorded using a Zeiss MZ16FA Stereo Microscope with a Leica DFC350 FX camera and Leica AF6000 software. Microscopic analysis of single cells taken from spots grown on solid media as above was performed by Differential Interference Contrast (DIC) microscopy using an Axioskop 2 mot plus (Zeiss) with a SPOT RT KE camera and spot software (Diagnostic Instruments).

Protein purification and in vitro analysis

A full description of protein purification is provided in the Supporting information. In brief, proteins were overproduced in E. coli with a TEV protease-cleavable His6 tag and isolated by Ni2+ affinity purification. If required, the His6 tag was cleaved using TEV protease and the protein re-isolated by reverse Ni2+ chromatography. A final SEC step was then always performed. For SEC analysis of complex formation, His6-tagged proteins (10 nmol each) in 50 mM Tris·HCl, pH 7.5, 250 mM NaCl were separated on a Superdex 75 10/300 GL column, calibrated using molecular weight standards (GE Healthcare). Quantitative SYPRO Orange staining was performed as described (Rickman et al., 2004), with image analysis using ImageJ. Molar ratios were the mean of at least four quantifications. ITC was performed in 50 mM Tris·HCl, pH 7.5, 250 mM NaCl at 30°C in a MicroCal iTC200 calorimeter. The sample cell contained 6 μM Rap1a dimer or Rap2a dimer and the syringe contained 120 μM Ssp1 or Ssp2. Titrations consisted of 30 × 8 μl injections of Ssp into Rap (or into buffer alone as control). Data analysis was performed with the Origin software provided (MicroCal). For affinity isolation of Ssp1 and Ssp2, 10 μg of His6-tagged Rap protein was immobilized on magnetic Ni2+ beads (Qiagen), incubated for 1 h with culture supernatant (after 7 h growth in LB), beads washed and bound proteins eluted by the addition of gel sample buffer. Identified proteins were excised from the Coomassie- (Ssp2) or Silver- (Ssp1) stained gel and identified by mass spectrometry.

Crystallographic analyses

Well-ordered trigonal and orthorhombic crystals of Rap1b and Rap2b, respectively, were obtained. The asymmetric unit for Rap1b consisted of a single subunit, while Rap2b displayed two dimers in the asymmetric unit. Diffraction data were recorded in-house and experimental phases were derived by single-wavelength anomalous diffraction measurements (Micossi et al., 2002), exploiting the signal from endogenous S atoms and I ions that had been added by soaking. The electron density maps were of high quality, and the models were completed, then refined to high resolution using standard methods (Dawson et al., 2008). Full crystallographic details are provided in the Supporting information and Table 1. Atomic co-ordinates and structure factors have been deposited in the Protein Data Bank (PDB) with accession codes 4AX2 (Rap1b) and 4B6I (Rap2b).

Acknowledgements

  1. Top of page
  2. Summary
  3. Introduction
  4. Results
  5. Discussion
  6. Experimental procedures
  7. Acknowledgements
  8. References
  9. Supporting Information

This work was supported by the Royal Society of Edinburgh (Personal Research Fellowship to S. J. C.), Medical Research Scotland (382 FRG), the Wellcome Trust [grants 082596, 083481, a PhD studentship (G. E.) and an ISSF award to the University of Dundee], the European Commission (FP7/2007-2013, the Aeropath project) and a Royal Society Project Grant (S. J. C.). We would like to thank Maximilian Fritsch, Sarah Murdoch, Matthias Trost, Emma Compton, Arnaud Javelle, Frank Sargent and members of the WNH lab for technical assistance and discussions.

References

  1. Top of page
  2. Summary
  3. Introduction
  4. Results
  5. Discussion
  6. Experimental procedures
  7. Acknowledgements
  8. References
  9. Supporting Information
  • Aubert, D.F., Flannagan, R.S., and Valvano, M.A. (2008) A novel sensor kinase-response regulator hybrid controls biofilm formation and type VI secretion system activity in Burkholderia cenocepacia. Infect Immun 76: 19791991.
  • Basler, M., Pilhofer, M., Henderson, G.P., Jensen, G.J., and Mekalanos, J.J. (2012) Type VI secretion requires a dynamic contractile phage tail-like structure. Nature 483: 182186.
  • Bonemann, G., Pietrosiuk, A., and Mogk, A. (2010) Tubules and donuts: a type VI secretion story. Mol Microbiol 76: 815821.
  • Burtnick, M.N., Brett, P.J., Harding, S.V., Ngugi, S.A., Ribot, W.J., Chantratita, N., et al. (2011) The cluster 1 type VI secretion system is a major virulence determinant in Burkholderia pseudomallei. Infect Immun 79: 15121525.
  • Cascales, E. (2008) The type VI secretion toolkit. EMBO Rep 9: 735741.
  • Cascales, E., and Cambillau, C. (2012) Structural biology of type VI secretion systems. Philos Trans R Soc Lond B Biol Sci 367: 11021111.
  • Choi, S.H., Lee, J.E., Park, S.J., Kim, M.N., Choo, E.J., Kwak, Y.G., et al. (2007) Prevalence, microbiology, and clinical characteristics of extended-spectrum beta-lactamase-producing Enterobacter spp., Serratia marcescens, Citrobacter freundii, and Morganella morganii in Korea. Eur J Clin Microbiol Infect Dis 26: 557561.
  • Chou, S., Bui, N.K., Russell, A.B., Lexa, K.W., Gardiner, T.E., Leroux, M., Vollmer, W., and Mougous, J.D. (2012) Structure of a peptidoglycan amidase effector targeted to Gram-negative bacteria by the Type VI secretion system. Cell Rep 1: 656664.
  • Cruickshank, D.W. (1999) Remarks about protein structure precision. Acta Crystallogr D Biol Crystallogr 55: 583601.
  • Dawson, A., Fyfe, P.K., and Hunter, W.N. (2008) Specificity and reactivity in menaquinone biosynthesis: the structure of Escherichia coli MenD (2-succinyl-5-enolpyruvyl-6-hydroxy-3-cyclohexadiene-1-carboxylate synthase). J Mol Biol 384: 13531368.
  • Ding, J., Wang, W., Feng, H., Zhang, Y., and Wang, D.C. (2012) Structural insights into the Pseudomonas aeruginosa type VI virulence effector Tse1 bacteriolysis and self-protection mechanisms. J Biol Chem 287: 2691126920.
  • Filloux, A., Hachani, A., and Bleves, S. (2008) The bacterial type VI secretion machine: yet another player for protein transport across membranes. Microbiology 154: 15701583.
  • Gerlach, R.G., and Hensel, M. (2007) Protein secretion systems and adhesins: the molecular armory of Gram-negative pathogens. Int J Med Microbiol 297: 401415.
  • Hood, R.D., Singh, P., Hsu, F., Guvener, T., Carl, M.A., Trinidad, R.R., et al. (2010) A type VI secretion system of Pseudomonas aeruginosa targets a toxin to bacteria. Cell Host Microbe 7: 2537.
  • Jani, A.J., and Cotter, P.A. (2010) Type VI secretion: not just for pathogenesis anymore. Cell Host Microbe 8: 26.
  • Kelley, L.A., and Sternberg, M.J. (2009) Protein structure prediction on the Web: a case study using the Phyre server. Nat Protoc 4: 363371.
  • Krissinel, E., and Henrick, K. (2007) Inference of macromolecular assemblies from crystalline state. J Mol Biol 372: 774797.
  • Laskowski, R.A., Watson, J.D., and Thornton, J.M. (2005) ProFunc: a server for predicting protein function from 3D structure. Nucleic Acids Res 33: W89W93.
  • Leiman, P.G., Basler, M., Ramagopal, U.A., Bonanno, J.B., Sauder, J.M., Pukatzki, S., et al. (2009) Type VI secretion apparatus and phage tail-associated protein complexes share a common evolutionary origin. Proc Natl Acad Sci USA 106: 41544159.
  • Li, M., Le Trong, I., Carl, M.A., Larson, E.T., Chou, S., De Leon, J.A., et al. (2012) Structural basis for type VI secretion effector recognition by a cognate immunity protein. PLoS Pathog 8: e1002613.
  • Lockhart, S.R., Abramson, M.A., Beekmann, S.E., Gallagher, G., Riedel, S., Diekema, D.J., et al. (2007) Antimicrobial resistance among Gram-negative bacilli causing infections in intensive care unit patients in the United States between 1993 and 2004. J Clin Microbiol 45: 33523359.
  • MacIntyre, D.L., Miyata, S.T., Kitaoka, M., and Pukatzki, S. (2010) The Vibrio cholerae type VI secretion system displays antimicrobial properties. Proc Natl Acad Sci USA 107: 1952019524.
  • Micossi, E., Hunter, W.N., and Leonard, G.A. (2002) De novo phasing of two crystal forms of tryparedoxin II using the anomalous scattering from S atoms: a combination of small signal and medium resolution reveals this to be a general tool for solving protein crystal structures. Acta Crystallogr D Biol Crystallogr 58: 2128.
  • Mulder, D.T., Cooper, C.A., and Coombes, B.K. (2012) Type VI secretion system-associated gene clusters contribute to pathogenesis of Salmonella enterica serovar Typhimurium. Infect Immun 80: 19962007.
  • Murdoch, S.L., Trunk, K., English, G., Fritsch, M.J., Pourkarimi, E., and Coulthurst, S.J. (2011) The opportunistic pathogen Serratia marcescens utilizes type VI secretion to target bacterial competitors. J Bacteriol 193: 60576069.
  • de Pace, F., Nakazato, G., Pacheco, A., de Paiva, J.B., Sperandio, V., and da Silveira, W.D. (2010) The type VI secretion system plays a role in type 1 fimbria expression and pathogenesis of an avian pathogenic Escherichia coli strain. Infect Immun 78: 49904998.
  • Petersen, T.N., Brunak, S., von Heijne, G., and Nielsen, H. (2011) SignalP 4.0: discriminating signal peptides from transmembrane regions. Nat Methods 8: 785786.
  • Petty, N.K., Foulds, I.J., Pradel, E., Ewbank, J.J., and Salmond, G.P. (2006) A generalized transducing phage (phiIF3) for the genomically sequenced Serratia marcescens strain Db11: a tool for functional genomics of an opportunistic human pathogen. Microbiology 152: 17011708.
  • Pukatzki, S., Ma, A.T., Revel, A.T., Sturtevant, D., and Mekalanos, J.J. (2007) Type VI secretion system translocates a phage tail spike-like protein into target cells where it cross-links actin. Proc Natl Acad Sci USA 104: 1550815513.
  • Pukatzki, S., McAuley, S.B., and Miyata, S.T. (2009) The type VI secretion system: translocation of effectors and effector-domains. Curr Opin Microbiol 12: 1117.
  • Rickman, C., Meunier, F.A., Binz, T., and Davletov, B. (2004) High affinity interaction of syntaxin and SNAP-25 on the plasma membrane is abolished by botulinum toxin E. J Biol Chem 279: 644651.
  • Rosales-Reyes, R., Skeldon, A.M., Aubert, D.F., and Valvano, M.A. (2012) The Type VI secretion system of Burkholderia cenocepacia affects multiple Rho family GTPases disrupting the actin cytoskeleton and the assembly of NADPH oxidase complex in macrophages. Cell Microbiol 14: 255273.
  • Russell, A.B., Hood, R.D., Bui, N.K., LeRoux, M., Vollmer, W., and Mougous, J.D. (2011) Type VI secretion delivers bacteriolytic effectors to target cells. Nature 475: 343347.
  • Russell, A.B., Singh, P., Brittnacher, M., Bui, N.K., Hood, R.D., Carl, M.A., et al. (2012) A widespread bacterial type VI secretion effector superfamily identified using a heuristic approach. Cell Host Microbe 11: 538549.
  • Sambrook, J., and Russell, D.W. (2001) Molecular Cloning: A Laboratory Manual, 3rd edn. Cold Spring Harbor, NY: Cold Spring Harbor Laboratory.
  • Schwarz, S., West, T.E., Boyer, F., Chiang, W.C., Carl, M.A., Hood, R.D., et al. (2010) Burkholderia type VI secretion systems have distinct roles in eukaryotic and bacterial cell interactions. PLoS Pathog 6: e1001068.
  • Suarez, G., Sierra, J.C., Erova, T.E., Sha, J., Horneman, A.J., and Chopra, A.K. (2010) A type VI secretion system effector protein, VgrG1, from Aeromonas hydrophila that induces host cell toxicity by ADP ribosylation of actin. J Bacteriol 192: 155168.
  • Wiseman, T., Williston, S., Brandts, J.F., and Lin, L.N. (1989) Rapid measurement of binding constants and heats of binding using a new titration calorimeter. Anal Biochem 179: 131137.
  • Yamaguchi, Y., and Inouye, M. (2011) Regulation of growth and death in Escherichia coli by toxin-antitoxin systems. Nat Rev Microbiol 9: 779790.
  • Zheng, J., and Leung, K.Y. (2007) Dissection of a type VI secretion system in Edwardsiella tarda. Mol Microbiol 66: 11921206.
  • Zou, T., Yao, X., Qin, B., Zhang, M., Cai, L., Shang, W., et al. (2012) Crystal structure of Pseudomonas aeruginosa Tsi2 reveals a stably folded superhelical antitoxin. J Mol Biol 417: 351361.

Supporting Information

  1. Top of page
  2. Summary
  3. Introduction
  4. Results
  5. Discussion
  6. Experimental procedures
  7. Acknowledgements
  8. References
  9. Supporting Information
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