Stenotrophomonas maltophilia responds to exogenous AHL signals through the LuxR solo SmoR (Smlt1839)

Abstract

Quorum Sensing (QS) mediated by Acyl Homoserine Lactone (AHL) molecules are probably the most widespread and studied among Gram-negative bacteria. Canonical AHL systems are composed by a synthase (LuxI family) and a regulator element (LuxR family), whose genes are usually adjacent in the genome. However, incomplete AHL-QS machinery lacking the synthase LuxI is frequently observed in Proteobacteria, and the regulator element is then referred as LuxR solo. It has been shown that certain LuxR solos participate in interspecific communication by detecting signals produced by different organisms. In the case of Stenotrophomonas maltophilia, a preliminary genome sequence analysis revealed numerous putative luxR genes, none of them associated to a luxI gene. From these, the hypothetical LuxR solo Smlt1839, here designated SmoR, presents a conserved AHL binding domain and a helix-turn-helix DNA binding motif. Its genomic organization—adjacent to hchA gene—indicate that SmoR belongs to the new family “LuxR regulator chaperone HchA-associated.” AHL-binding assays revealed that SmoR binds to AHLs in-vitro, at least to oxo-C8-homoserine lactone, and it regulates operon transcription, likely by recognizing a conserved palindromic regulatory box in the hchA upstream region. Supplementation with concentrated supernatants from Pseudomonas aeruginosa, which contain significant amounts of AHLs, promoted swarming motility in S. maltophilia. Contrarily, no swarming stimulation was observed when the P. aeruginosa supernatant was treated with the lactonase AiiA from Bacillus subtilis, confirming that AHL contributes to enhance the swarming ability of S. maltophilia. Finally, mutation of smoR resulted in a swarming alteration and an apparent insensitivity to the exogenous AHLs provided by P. aeruginosa. In conclusion, our results demonstrate that S. maltophilia senses AHLs produced by neighboring bacteria through the LuxR solo SmoR, regulating population behaviors such as swarming motility.

Introduction

Bacterial cells can communicate with each other to facilitate their rapid adaptation to fluctuations in the environment. This cell-cell communication mechanism, known as quorum sensing (QS), relies primarily on the production, detection, and response to diffusible signal molecules (also called autoinducers) in a cell-density dependent manner (Fuqua et al., 1994; Whitehead et al., 2001; Fuqua and Greenberg, 2002; Federle and Bassler, 2003). Through this QS communication, numerous bacterial species regulate a variety of functions such as biofilm formation, motility, antibiotic resistance, toxin production, exopolysaccharide synthesis, and extracellular enzyme production among others (Miller and Bassler, 2001). In Gram-negative bacteria, N-acyl homoserine lactones (AHLs) are to date the most extensively and best characterized QS signaling molecules. AHL-QS regulation consists of a LuxI-type synthase, which produces signal molecules, and a LuxR-type receptor that binds AHLs and regulates expression of certain genes when signal concentration reaches a critical threshold. LuxR regulators are about 250 residues in length and present two typical domains, the N-terminal autoinducer AHL binding domain (Shadel et al., 1990; Slock et al., 1990) and the C-terminal helix-turn-helix (HTH) DNA-binding domain (Choi and Greenberg, 1991; Fuqua and Winans, 1994). In the presence of AHLs, the N-terminal binding domain interacts with the signal molecule, habilitating the DNA-binding domain to induce transcription of certain genes by binding to their promoters in a region named luxR box (Devine et al., 1989; Stevens and Greenberg, 1997). The DNA-binding domain includes three highly conserved aminoacids, while the AHL-binding domain presents six hydrophobic or aromatic residues displaying remarkable variability (18-25%) (Zhang et al., 2002).

The increasing availability of bacterial genome sequences has led to the identification of several LuxR and LuxI homologs. Typically, both luxI-type and luxR-type genes are located adjacent in the bacterial genome (the cognate luxR/I pair). However, luxR-type genes without a cognate luxI-type in their vicinity are frequently found, and these regulatory elements are then called “orphan” (Fuqua, 2006) or “solo” LuxR (Subramoni and Venturi, 2009a). Recent studies have revealed that “luxR solo” genes are widely distributed among bacterial genomes (Hudaiberdiev et al., 2015). LuxR solos present the same modular organization as canonical LuxR, displaying the N-terminal and C-terminal domains. The nature of the signal molecules that bind to the different LuxR solos is quite heterogeneous. It has been shown that the LuxR solo QscR from Pseudomonas aeruginosa bind to self-produced AHL signals (Chugani et al., 2001; Lequette et al., 2006), while SdiA of Salmonella enterica and Escherichia coli respond to exogenous AHL signals (Ahmer et al., 1998; Michael et al., 2001; Ahmer, 2004; Yao et al., 2006). Interestingly, the LuxR solo OryR from Xanthomonas oryzae pv. oryzae interacts with plant signals, in particular those produced by rice (Ferluga et al., 2007; Ferluga and Venturi, 2009; González et al., 2013). More recently, it has been reported that the human and insect pathogen Photorhabdus asymbiotica contains a LuxR solo PauR that is the regulator element of a new QS-system, which is mediated by dialkylresorcinols (DARs) and cyclohexanediones (CHDs) signals (Brameyer et al., 2015). Altogether, this shows that LuxR solos can participate in a wide variety of signaling networks.

Stenotrophomonas maltophilia is an ubiquitous gram-negative bacterium considered an emerging nosocomial pathogen (Brooke, 2012). Moreover, it is frequently found in lungs of cystic-fibrosis (CF) patients (Demko et al., 1998), usually co-isolated with P. aeruginosa (Moskowitz et al., 2005). The QS described in S. maltophilia is based on the signaling molecule DSF (11-cis-2-decenoic acid), by which it regulates virulence-related processes (Fouhy et al., 2007; Huedo et al., 2014). To date, no S. maltophilia strain has been reported to produce AHL and the K279a reference genome contains no luxI homolog (Crossman et al., 2008), at least of the usual luxI types (Waters and Bassler, 2005). However, sequence analysis reveals that this genome encodes a total of 15 putative LuxR-like proteins, based mainly on homologies of the DNA-binding response domain. From these, only the LuxR solo Smlt1839 showed an N-AHL autoinducer-binding domain. The objective of our study has been to experimentally investigate the role of Smlt1839 in AHL binding and swarming regulation in S. maltophilia, in the presence of exogenous and heterologous AHLs.

Materials and methods

Bacterial strains and growth conditions

Bacterial strains used in this study are listed in Table 1. E. coli strains DH5a and BL21 (DE3) were used for general cloning purposes and overexpression of smoR, respectively. S. maltophilia E77 (Ferrer-Navarro et al., 2013) was used as a model strain to investigate the role of SmoR in detection and response of exogenous AHL signals. P. aeruginosa MPAO1 strain was used as an AHL-producer bacterium to evaluate the effect of exogenous signal molecules on swarming motility of S. maltophilia. Agrobacterium tumefaciens KYC55 (Zhu et al., 2003) was used as a reporter strain to detect AHL production.

Table 1.

Primers used in this study.

Primer	Sequence (5′-3′)	Restriction site
P1MutSmoR	AAGCTTTGCCCGGTTCGGTATCGG	HindIII
P2MutSmoR	GGATCCTCGCGGCGAGGCACTTCC	BamHI
P3MutSmoR	GGATCCCCGGTTCAGCGCCCGGCC	BamHI
P4MutSmoR	GAATTCCCCAGCCGCCAGCCCAGC	EcoRI
PErm5′	GGATCCGAAACGTAAAAGAAGTTATG	BamHI
PErm3′	GGATCCTACAAATTCCCCGTAGGC	BamHI
PErm5′rev	GATACTGCACTATCAACACAC	–
PErm3′rev	CTTCCAAGGAGCTAAAGAGGT	–
P1DemSmoR	GTACGTCGGGCGTATCG	–
P2DemSmoR	GCCCTTCTATGCTGG	–
P1ProSmoR	TCTAGACGCACACGCATGGACCG	XbaI
P2ProSmoR	GGATCCGAAGGCGTCGCGCTCGG	BamHI
P1ExpSmoR	CATATGAGCGATCTGGTGCAGGCG	NdeI
P2ExpSmoR	CTCGAGTCAGTCTTCGATCTCGCCT	XhoI
PT7up	TAATACGACTCACTATAGGG	–
PT7dw	GCTAGTTATTGCTCAGCGG	–

E. coli, S. maltophilia and P. aeruginosa strains were routinely grown in Luria-Bertani (LB) medium at 37°C. A. tumefaciens KYC55 was grown in AT medium (Fuqua and Winans, 1994) at 30°C. When required, the antibiotics were supplemented as follows: ampicillin (Ap) 20 μg/ml (E. coli); tetracycline (Tc) 17 μg/ml (E. coli and P. aeruginosa) or 2 μg/ml (A. tumefaciens); erythromycin (Erm) 50 μg/ml (E. coli) or 500 μg/ml (S. maltophilia); gentamicin (Gm) 10 μg/ml (E. coli), 100 μg/ml (A. tumefaciens) or 40 μg/ml (S. maltophilia); and spectinomycin (Spc) 100 μg/ml (E. coli and A. tumefaciens).

Sequence determination and in silico analysis

A 5.5 kb fragment containing the ORFs of smlt1840 and smlt1839 plus their flanking regions was amplified from S. maltophilia strain E77 genomic DNA and subsequently sequenced (Macrogen). The sequence has been used for sequence alignments as well as reference to generate a ΔsmoR mutant in this model strain. The fragment corresponding to hchA-smoR operon and its predicted promoter (1658 bp) was submitted to Genbank under the accession number KP691985. Annotation was done using BLAST (Altschul et al., 1990) and intergenic regions were manually inspected for palindromic motifs and cis elements that participate in regulating translation. Program RSAT (Thomas-Chollier et al., 2011) was used to scan for a pattern (the palindromic box) within all ORF upstream regions in the K279a genome. A simple screen for luxR-like genes using a S. maltophilia K279a genomic sequence (AM743169.1) was done by using BLAST and PSI-BLAST (Altschul et al., 1997) to detect remote homologs. Sequences of the hchA-smoR operon from other S. maltophilia strains were retrieved from their genome sequences at NCBI (http://www.ncbi.nlm.nih.gov/genome/). Translation of ORFs to amino-acid sequences and sequence alignments were done with MEGA 6 (Tamura et al., 2013) and then analyzed with SMART (Letunic et al., 2009) for the identification and annotation of protein domains. Nucleotide and protein sequences were aligned using the ClustalW module implemented in MEGA 6 and manually edited and visualized with BioEdit. Software was run with default parameters unless otherwise stated. Identification of “LuxR-like regulators chaperone HchA associated” in other Proteobacteria was predicted by InterPro (http://www.ebi.ac.uk/interpro/) (Mitchell et al., 2014).

Preparation of fusion and expression vectors

Oligonucleotides used as primers and plasmids used in this study are listed in Tables 2 and 3, respectively. The transcriptional fusion construct for the smoR promoter in pBBR1MCS-5-lacZ (Fried et al., 2012) was generated by amplifying a fragment of 415 bp containing the putative promoter of the operon hchA-smoR (smlt1840-smlt1839) from S. maltophilia E77, using primers P1ProSmoR and P2ProSmoR and FastStart DNA polymerase (Roche). The fragment was digested using XbaI and BamHI and cloned into their respective restriction sites into pBBR5MCS-5-lacZ, generating pBBR5MCS-PsmoR::LacZ. This vector was electroporated (Choi et al., 2006) into S. maltophilia E77 and transformants were seeded onto LB plates supplemented with 40 μg/ml Gm.

Table 2.

Plasmids used in this study.

Plasmid	Relevant Characteristics	Source
pGEM-Erm	Cloning vector carrying Erm resistance gene, Ampr, Ermr	This work
pEX18Tc	Suicide allelic exchange vector; Tcr	Hoang et al., 1998
pEXsmoR	pEX18Tc carrying E77 smoR flanking regions interrupted with Erm resistance gene, Tcr, Ermr	This work
pBBR1MCS-5	Broad-host-range cloning vector, Gmr	Kovach et al., 1995
pET22b	IPTG inducible expression vector, Ampr	Novagen
pET22b-smoR	IPTG inducible expression vector carrying smoR ORF, Ampr	This work
pBBR1MCS-5-lacZ	pBBR1MCS-5 plasmid carrying promoterless lacZ gene, Gmr	Fried et al., 2012
pBBR1MCS-5-PsmoR::lacZ	pBBR1MCS-5 plasmid carrying fusion PsmoR::lacZ gene, Gmr	This work
pME6000	Broad-host-range cloning vector, Tcr	Maurhofer et al., 1998
pMEPlac::aiiA	pME6000 carrying lactonase aiiA gene from B. subtilis under the control of Plac promoter, Tcr	Reimmann et al., 2002

Table 3.

Strains used in this study.

Strains	Relevant characteristics	References
S. maltophilia
E77	Wild type	Ferrer-Navarro et al., 2013
E77 ΔsmoR	E77 ΔsmoR (Δsmlt1839), Ermr	This work
E77 pBBR1MCS-5-lacZ	E77 harboring vector pBBR1MCS-5-lacZ, Gmr	This work
E77 pBBR1MCS-5-PsmoR::lacZ	E77 harboring vector pBBR1MCS-5-PsmoR::lacZ, Gmr,	This work
E77 ΔsmoR pBBR1MCS-5-lacZ	E77 ΔsmoR harboring vector pBBR1MCS-5-lacZ, Gmr, Ermr	This work
E77 ΔsmoR pBBR1MCS-5-PsmoR::lacZ	E77 ΔsmoR harboring vector pBBR1MCS-5-PsmoR::lacZ, Gmr, Ermr	This work
E. coli
DH5α	recA1 endA1 hsdR17 gyrA96 supE44 thi-1 relA1Δ(lacZYA-argF)U169 deoR Φ80dlacZΔM15	Lab. Collection
DH5α pEXsmoR	DH5α harboring vector pEXsmoR, Tcr, Ermr	This work
BL21 (DE3)	fhuA2 [lon] ompT gal (λ DE3) [dcm] ΔhsdSλ DE3 = λ sBamHIo ΔEcoRI-B int::(lacI::PlacUV5::T7 gene1) i21 Δnin5	Novagen
BL21 (DE3) pET22b	BL21 (DE3) harboring pET22b, Ampr	This work
BL21 (DE3) pET22b-smoR	BL21 (DE3) harboring pET22b-smoR, Ampr	This work
P. aeruginosa
MPAO1	Wild type	Jacobs et al., 2003
MPAO1 pME600	MPAO1 harboring pME600, Tcr
MPAO1 pMEPlac::aiiA	MPAO1 harboring pME-Plac::aiiA, Tcr	This work
A. tumefaciens
KYC55	KYC55 harboring vectors pJZ384, pJZ410 and pJZ372 Spcr, Gmr, Tcr	Zhu et al., 2003

To generate the expression vector for SmoR production in E. coli, the ORF of smlt1839 was amplified using primer pair P1ExpSmoR-P2ExpSmoR and the amplified fragment was digested with NdeI and XhoI and cloned into their respective restriction sites into pET22b (Novagen), creating pET22b-smoR. E. coli strain BL21 (DE3) was transformed (Sambrook et al., 1989) with plasmid pET22b-smoR and transformants were seeded onto LB plates containing 20 μg/ml Amp.

The vectors pME6000 (Maurhofer et al., 1998) and pMElacZ::aiiA (Reimmann et al., 2002)—the latter carrying a transcriptional fusion between lacZ promoter and the ORF of the lactonase AiiA from Bacillus subtilis strain A24 (Dong et al., 2000)—were provided by the authors and were used to investigate the effect of the lactonase AiiA on the degradation of the AHL signals from P. aeruginosa. Both vectors were electroporated (Choi et al., 2006) into P. aeruginosa MPAO1 and transformants were seeded onto LB plates containing 17 μg/ml Tc.

Generation of ΔsmoR mutant

S. maltophilia E77 ΔsmoR mutant was obtained by allelic-exchange recombination using erythromycin as antibiotic-resistance cassette. Briefly, smoR upstream and downstream flanking regions (993 and 863 bp, respectively) were amplified by PCR using primer pairs P1MutSmoR-P2MutSmoR (upstream region) and P3MutSmoR-P4MutSmoR (downstream region) and inserted, flanking an erythromycin cassette, into the suicide vector pEX18Tc (Hoang et al., 1998), generating plasmid pEXsmoR. The erythromycin cassette was previously amplified from plasmid pGEM-Erm (Table 2) using primers PErm5′ and PErm3′. S. maltophilia E77 was electroporated (Choi et al., 2006) with the suicide vector pEXsmoR and transformants were seeded onto LB plates containing 500 μg/mL Erm and subsequently streaked onto LB plates containing 17 μg/mL Tc to discard single cross-over events. smoR deletion was also verified by PCR using primer combinations P1DemSmoR-PErm5′rev (for upstream region) and P2DemSmoR-PErm3′rev (for downstream region). The obtained fragments were subsequently verified by sequencing (Macrogen).

Measuring ß-galactosidase activity

To evaluate the expression levels of hchA-smoR promoter, ß-galactosidase assays were performed for the strains E77 wild type and ΔsmoR mutant harboring either the vectors pBBR1MCS-5-PsmoR:lacZ or pBBR1MCS-5-lacZ—the latter used as a control– during growth in LB medium at 30°C, following the protocol described by Miller (1972). All bacterial cultures were started with an initial inoculum corresponding to an optical density at 550 nm (OD₅₅₀) of 0.05. To determine the activity of the hchA-smoR promoter during growth curve, 0.1 ml-samples were taken at different times from 4 to 48 h. To investigate the effect of the presence of AHL molecules in the activity of the hchA-smoR promoter, initial cultures were supplemented with various synthetic AHLs (Cayman Chemical) –C6-HSL, oxo-C8-HSL, C8-HSL, and C10-HSL– with different concentrations (1 up to 10 μM), and 0.1 ml samples were taken and measured after 24 h and 48 h of incubation at 30°C. After analyzing the data we determined β-galactosidase specific activities in Miller Units (Miller, 1972). All AHL stocks were solubilized in 70% acetonitrile/water acidified with 0.1 M HCl final concentration. All experiments were performed by triplicate and comparison of ß-galactosidae activity was performed by One-Way analysis of variance (ANOVA) with a Bonferroni's multiple comparison post-test.

Extraction, thin layer chromatography and bioassay of AHLs

To evaluate AHL produced by P. aeruginosa, 150 ml culture supernatants of strain MPAO1, or MPAO1 transformed with either pME6000 or pMElacZ::aiiA grown in LB at 37°C for 24 h (OD₅₅₀ of about 2), were extracted with 300 ml of acidified ethyl acetate (0.1% acetic acid). The organic phase was evaporated to dryness using a rotary evaporator, and the residues were dissolved in an appropriate volume of acidified ethyl acetate. 5 μl aliquots of dissolved ethyl acetate residues were spotted onto C18 reverse-phase plate (Merck) (Shaw et al., 1997) and separated with methanol:water (60:40, vol/vol) as running solvent. TLC plates were subsequently air-dried for at least 1 h and overlaid with 100 ml of unsolidified warm AT medium containing 0.8% agar, 60 μg/ml X-Gal and the AHL reporter strain KYC55 to an OD₅₅₀ of ca. 0.8. TLC plates were incubated overnight at 30°C, and AHL activity was identified by the presence of blue spots. 2 μl of the aforementioned synthetic AHLs were also tested in TLC coupled to bioassay and used as a control.

AHL binding assay

The AHL binding assay was performed as described (Subramoni and Venturi, 2009b), with few modifications. 20 ml cultures of E. coli BL21 (DE3) harboring either pET22b or pET22b-smoR were grown at 37°C in LB medium containing 10 μg/ml Amp to an OD₅₅₀ of 0.1. Bacterial cultures were then supplemented with different AHL molecules (C6-HSL, oxo-C8-HSL, C8-HSL and C10-HSL) at 10 and 20 μM final concentration and cultures were incubated until reaching an OD₅₅₀ of 0.6. SmoR production was induced with 1 μM final concentration of IPTG and the cultures were additionally incubated for 3.5 h. OD₅₅₀ was measured and the cultures were adjusted to contain an equal number of cells per mL and subsequently centrifuged. Cell pellets were washed three times with 10 ml of PBS and cellular suspensions were extracted twice with the same volume of acidified ethyl acetate. The extracts were then dried, dissolved in ethyl acetate and analyzed by TLC coupled to AHL bioassay, as described above. An aliquot of the corresponding induced culture was previously removed to control the identity of the overproduced recombinant protein (see Supplementary Figure S1).

Swarming assay

Swarming motility was assayed on BM2 medium plates (62 mM potassium phosphate buffer, pH = 7, 2 mM MgSO₄, 10 μM FeSO₄, 0.5% [wt/vol] casamino acids, supplemented with glucose 0.4% and solidified with 0.5% BD Difco Noble agar) (Overhage et al., 2007). Plates containing 20 ml of fresh swarm medium were dried under a laminar-flow hood for 20 min before pin-inoculation. When indicated, solidified swarm plates were supplemented with 10 μl of concentrated culture supernatant—extracted as described above– of P. aeruginosa MPAO1 and its derivative strains, as indicated in figure captions. Inoculated swarm plates were sealed to maintain the humidity and incubated at 30°C up to five days. Swarming experiments were done in triplicate and representative images are shown.

Results

Smlt1839 contains both the AHL- and DNA-binding LuxR domains

It is known that certain non AHL-producing bacteria are able to sense AHLs and regulate various biological functions in response to signals produced by others through diverse LuxR-like regulators (Patankar and González, 2009). The genome of S. maltophilia strain K279a (Crossman et al., 2008) was revisited for the presence of genes encoding putative LuxR-like regulators. Besides the eight genes already annotated as two-component-system response regulators of the LuxR family, a total of seven additional hypothetical LuxR regulators were identified (Table 4), none of them associated to a luxI homolog. All these LuxR-solo candidates were examined in detail for the presence of the typical N-terminal AHL-binding domain (PFAM 03472) and the C-terminal helix-turn-helix (HTH) DNA-binding domain (PFAM 00196) (Miller and Bassler, 2001). From these, only the gene smlt1839 was found to encode for a protein—here named SmoR (Stenotrophomonas maltophilia orphan regulator)—containing both conserved domains (Table 4). A subsequent protein alignment with known orphan regulators from distinct Proteobacteria including PpoR from P. putida, SdiA from S. enterica, OryR from X. oryzae pv. oryzae, and TraR from A. tumefaciens, revealed that at the N-terminal domain four out of six residues involved in AHL binding (Patankar and González, 2009) are conserved in SmoR (Figure 1). Concerning the C-terminal HTH domain, the three residues responsible for DNA binding (Hanzelka and Greenberg, 1995; Fuqua et al., 1996) are also conserved in SmoR (Figure 1). Further protein BLAST analysis revealed that SmoR is largely conserved among S. maltophilia (data not shown). These results suggest that the conserved regulator SmoR (Smlt1839) could be implicated in signaling systems in S. maltophilia.

Table 4.

Hypothetical LuxR-like regulators annotated in the genome of S. maltophilia strain K279a.

Locus ID	Lenght	N-ter Domain	C-ter Domain	Annotation in K279a
Smlt1839	234	AHL	LuxR HTH	LuxR family transcriptional regulator
Smlt0195	212	REC	LuxR HTH	LuxR family two component response regulator
Smlt0389	223	REC	LuxR HTH	Two component transcriptional regulator, LuxR family
Smlt2299	210	REC	LuxR HTH	Response regulator protein LuxR family
Smlt2366	208	REC	LuxR HTH	Two-component response regulator, LuxR family
Smlt4224	212	REC	LuxR HTH	LuxR family two-component response regulator
Smlt0367	200	REC	LuxR HTH	Two-component system response regulator, LuxR family
Smlt0400	254	REC	LuxR HTH	Two-component response regulator transcriptional regulator
Smlt0881	213	REC	LuxR HTH	Two-component response regulator transcriptional regulator
Smlt1255	213	REC	LuxR HTH	Two-component response regulator transcriptional regulator
Smlt1788	215	REC	LuxR HTH	Two-component response regulator transcriptional regulator
Smlt2595	224	REC	LuxR HTH	Two-component response regulator transcriptional regulator
Smlt2658	213	REC	LuxR HTH	Two-component response regulator transcriptional regulator
Smlt2891	217	REC	LuxR HTH	Two-component response regulator transcriptional regulator
Smlt4624	221	REC	LuxR HTH	Two component system response regulator

Figure 1.

Protein alignment of orthologs LuxR solos from diverse Proteobacteria; PpoR (FM992078): Pseudomonas putida strain RD8MR3; SdiA (AAC08299.1): Salmonella enterica subsp. enterica serovar Typhimurium strain LT2; OryR (AAR91700.1): Xanthomonas oryzae pv. oryzae; TraR (AAZ50597.1): A. tumefaciens; SmoR: S. maltophilia E77 (KP691985). Red boxes highlight amino acids implicated in AHL binding and yellow boxes indicate residues involved in DNA binding (HTH). From these, conserved amino acids in E77 are marked with an asterisk.

S. maltophilia SmoR binds AHLs

It has been demonstrated that various LuxR solos containing the AHL-binding domain are able to bind to one or more AHL signal molecules. To determine whether in S. maltophilia the regulator SmoR could bind to any of these signals, an AHL-binding assay was performed. The appropriate overexpression of S. maltophilia smoR in E. coli strain BL21 (DE3) was validated by MALDI-MS analysis prior to initiate the AHL-binding assay (see Supplementary Figure S1).

E. coli BL21 (DE3) harboring either the empty vector pET-22b or the one overproducing SmoR were grown in a rich medium supplemented with a variety of AHLs (see Materials and Methods). After the appropriate incubation time, the culture supernatant was removed and the cell pellet was washed and subsequently extracted with acidified ethyl acetate. Concentrated cell extracts were visualized by TLC coupled to the AHL bioassay, resulting in the detection of the signal oxo-C8-HSL (Figure 2). Likewise, it was observed that the detection depends on AHL concentration, since the culture supplemented with 20 μM oxo-C8-HSL presented a more intense spot compared to that supplemented with 10 μM. On the other hand, cell extracts from E. coli cells containing the empty vector did not show detectable AHL activity (Figure 2). The experiment was performed by triplicate and non-systematic binding was observed for the other AHLs tested. Overall, this indicates that S. maltophilia could sense AHL signal molecules –in particular oxo-C8-HSL– through the LuxR solo SmoR.

Figure 2.

Representative image of AHL binding assay done for E. coli BL21 (DE3) harboring the expression vector pET22b-smoR or the empty vector pET22b grown in LB supplemented with AHLs at concentration of either 10 or 20 μM. Blue spots correspond to AHL signal. oxo-C8-HSL was used as control.

hchA and smoR are part of the same operon, and operon expression is growth-phase- and AHL-dependent

In S. maltophilia K279a, the gene encoding the regulator SmoR is localized downstream of the gene encoding for the chaperone HchA (Smlt1840), separated by only five nucleotides, indicating that both genes could form the operon hchA-smoR. This genetic organization is conserved in all available S. maltophilia genomes and also in the clinical strain E77 used in the present study. The upstream genes to hchA in strains D457 and JV3 are oriented in the opposite direction, indicating that there must be a promoter preceding hchA and confirming the existence of a bicistronic operon. Interestingly, this operon has been observed only in few Gammaproteobacteria, including Pseudomonas spp., Vibrio spp., Acinetobacter spp., Serratia spp., among few others, as predicted by InterPro (Family IPR019941). Accordingly, these regulator elements are annotated as “LuxR chaperone HchA-associated”. In E. coli, the gene hchA encodes for the chaperone Hsp31, which displays a high protein identity (60%) to S. maltophilia HchA. However, E. coli hchA is an isolated gene in this bacterial genome. It has been shown that Hsp31 is a glyoxalase that plays a central role in detoxification of dicarbonyl radicals (Subedi et al., 2011) as well as in the response to bacterial stress such as heat shock (Mujacic et al., 2004; Mujacic and Baneyx, 2006) and acidic conditions (Mujacic and Baneyx, 2007). In these mentioned studies it has been reported that transcription of hchA is induced at high population density.

In S. maltophilia E77 the upstream hchA-smoR operon region was examined for the presence of a putative promoter. Despite canonical core promoter elements are not found in this region, DNA sequence alignment of this region from different S. maltophilia strains revealed a conserved ribosome-binding site and a palindromic conserved motif spanning from positions −75 to −56 with respect to the translational start site (Figure 3A). The genome of S. maltophilia K279a was also evaluated for the presence of this palindromic motif in other promoter gene regions. Curiously, only a highly similar box (68.75% identity) was found in the intergenic region between smlt2137 (position −143 to −159) and smlt2138 (position −15 to −31). Those genes encode for a universal stress-family protein (Smlt2137) and for the transcriptional regulator NfxB (Smlt2138) (Shiba et al., 1995), respectively.

Figure 3.

(A) Alignment of the hchA-smoR promoter from different S. maltophilia strains. Gray shadow indicates the palindromic motif. Underlined sequences correspond to the putative ribosome binding site (RBS) and the start codon (ATG). (B) ß-galactosidase assay expressed in Miller Units of E77 WT and ΔsmoR mutant both harboring either pBBR1MCS-5::lacZ or pBBR1MCS-5-PsmoR::lacZ monitored during 48 h. Under these conditions all tested strains showed similar growth curves. (C) ß-galactosidase activity of E77 wild type and ΔsmoR mutant both harboring vector pBBR1MCS-5-PsmoR::lacZ grown in LB supplemented with diverse AHLs at 1 μM concentration each and incubated at 30°C for 24 or 48 h. Relative expression values are reported as Miller units of β-galactosidase activity in cells grown under the indicated growth conditions divided by the values in cells grown in LB broth without AHLs. ^*P < 0.05; ^**p < 0.01.

The hchA-smoR upstream region including the palindromic sequence motif was fused to lacZ gene and used in ß-galactosidase experiments to corroborate the existence of a promoter. The expression levels of the fusion construct PsmoR::lacZ were monitored in S. maltophilia strain E77 wild type and its derivative ΔsmoR mutant, in order to determine whether the expression pattern of the operon was similar to that previously described for the hchA gene in E. coli (Mujacic and Baneyx, 2006, 2007). Additionally, the role of SmoR in such expression was also evaluated, since the autoregulation of LuxR proteins is relatively common (Shadel and Baldwin, 1992; Chatterjee et al., 1996; Minogue et al., 2002).

The results from the ß-galactosidase experiments indicate that the promoter activity is slight at low cell densities and increases with bacterial-growth rate, showing a maximum at 48 h (stationary phase, Figure 3B). Although this tendency was observed in both wild type and ΔsmoR backgrounds, the absence of SmoR led to increased levels of expression compared to the wild type strain E77, specially at late stationary phase of growth (Figure 3B) (P < 0.01). Under these standard conditions (LB and 30°C) all tested strains showed similar growth curves reaching stationary phase by 24 h approximately. These results suggest that operon components would act at high cell densities, participating likely in this sort of stress response as observed for Hsp31 in E. coli.

Since we observed in vitro that SmoR bind the signal oxo-C8-HSL (Figure 2) and it is known that some active LuxR-like proteins can autoregulate their own expression, we wanted to investigate the role of SmoR on the regulation of hchA-smoR operon expression in the presence of AHLs. To do that, β-galactosidase assays were performed for the same strains supplemented with various AHLs (see Materials and Methods). The results showed that the expression of the operon was also modulated by the presence of these signal molecules. In particular, supplementation of E77 wild type with 1 μM C8-HSL resulted into approximately threefold and 8-fold operon activation at 24 and 48 h post induction respectively, compared to the expression levels of the supplemented ΔsmoR mutant (Figure 3C). This indicates that SmoR is involved in AHL-dependent operon-expression regulation.

AHLs produced by P. aeruginosa promote swarming motility in S. maltophilia, SmoR playing a central role in this stimulation

It is known that AHL signals modulate several biological functions not only in AHL-producing bacteria, but also in certain species lacking typical luxI/luxR systems which are still able to respond to exogenous AHLs through diverse orphan LuxR. One of the behaviors that have raised more interest recently and is commonly regulated by AHL-QS is swarming motility (Daniels et al., 2004). Swarming motility is a rapid and coordinated translocation of a bacterial population across semi-solid surfaces, which frequently requires quorum sensing-mediated synchronization (Kearns, 2010).

Since S. maltophilia frequently cohabit with AHL-producing bacteria –i.e., P. aeruginosa (Moskowitz et al., 2005)– we investigated the effect that P. aeruginosa AHLs could have on S. maltophilia regulation, more specifically on swarming motility. To that end, we supplemented S. maltophilia swarming plates with concentrated supernatants of P. aeruginosa strain MPAO1 wild type and MPAO1 harboring the plasmid pMEPlac::aiiA, which expresses the lactonase AiiA from B. subtilis (Dong et al., 2000). In order to corroborate the effect of the lactonase AiiA in AHL degradation, TLC followed by AHL bioassay was performed in parallel to swarming assays. As shown in Figure 4, expression of AiiA led to a decrease of P. aeruginosa AHL production and, interestingly, it resulted in a drastic reduction of S. maltophilia swarming stimulation. These results would indicate that AHL signals produced by P. aeruginosa promote swarming motility in S. maltophilia.

Figure 4.

Representative images of (A) TLC coupled to AHL bioassay of concentrated supernatants of P. aeruginosa MPAO1, MPAO1 pMEPlac::aiiA, and MPAO1 pME6000. Blue spots correspond to AHL molecules. (B) Swarming motility in BM2 0.5% agar medium plates of S. maltophilia E77 supplemented with 10 μl of the same concentrated supernatants (SN) and incubated at 30°C for 5 days.

Several evidences drive us to suggest that SmoR was responsible for the observed AHL-mediated swarming stimulation in S. maltophilia strain E77. It has been shown that, in the related bacteria X. oryzae pv. oryzae, the LuxR solo OryR also regulates certain motility processes, including swarming (González et al., 2013). In order to test such hypothesis in S. maltophilia, MPAO1 concentrated supernatants were spotted onto swarming plates seeded with the strains E77 wild type and the ΔsmoR mutant. The results further demonstrate that, as observed before, the MPAO1 concentrated supernatant significantly promotes the swarming ability of E77 (Figure 5). To the contrary, mutation of smoR resulted into a loss of swarming motility and supplementation with P. aeruginosa concentrated supernatant produced only a minor stimulation compared to E77 WT, perhaps due to the surfactant character of the AHL signals and other hydrophobic molecules present in its supernatant. These results strongly suggest that AHLs produced exogenously promote swarming motility in S. maltophilia and SmoR plays a central role in such stimulation (Figure 5).

Figure 5.

Representative images of swarming motility in BM2 0.5% agar medium plates of S. maltophilia E77 WT and ΔsmoR mutant supplemented with 10 μl of concentrated supernatants (SN) of P. aeruginosa strain MPAO1 WT and incubated at 30°C for 5 days. The white cross indicates the zone of the addition of the concentrated supernatants.

Discussion

The interest in LuxR-solo investigation has grown among microbiologists, since these regulatory elements may unveil novel signaling systems. The increment of public sequenced genomes has permitted scientists to screen an extraordinary number of bacterial genomes and identify new regulator elements. It recently has been shown in bacteria that 75% of the annotated luxR-type genes encode for a “LuxR solo” (Hudaiberdiev et al., 2015), which is a surprisingly high proportion. To date, it is known that various LuxR can regulate a range of biological function in response to: endogenous AHLs (Chugani et al., 2001; Lequette et al., 2006); exogenous AHLs produced by neighboring bacteria (Ahmer et al., 1998; Michael et al., 2001; Ahmer, 2004; Yao et al., 2006); the novel bacterial signaling molecules dialkylresorcinols (DARs) and cyclohexanediones (CHDs) (Brameyer et al., 2015); or even signals produced by plants (Ferluga et al., 2007; Ferluga and Venturi, 2009). Considering the high heterogeneity and complexity of LuxR solos in bacteria, it is highly probable that new regulatory networks are there to discover.

The aim of the present study was to identify and investigate putative LuxR solos in S. maltophilia. After screening the genome of the model strain K279a (Crossman et al., 2008), only the protein encoded by the smlt1839 gene (SmoR) was found to display the two typical LuxR domains: the autoinducer-binding domain (Shadel et al., 1990; Slock et al., 1990) and the DNA-binding helix-turn-helix (HTH) domain (Choi and Greenberg, 1991; Fuqua and Winans, 1994). Analysis at the amino-acid sequence level revealed that from the 9 crucial residues (Whitehead et al., 2001; Zhang et al., 2002), seven are conserved in SmoR. Diverse structural and functional analyses of several LuxR regulators have revealed that, while the DNA-binding domain (HTH) is widely conserved, the autoinducer-binding domain presents substantial variability, likely to adjust to a range of signal molecules (Vannini et al., 2002; Zhang et al., 2002; Yao et al., 2006; Bottomley et al., 2007). This is the situation observed in S. maltophilia SmoR, where the AHL-binding domain presents substitutions in residues 62 and 74, while the HTH domain is perfectly conserved (Figure 1). It has been reported that in A. tumefaciens, the LuxR solo TraR also binds to oxo-C8-HSL through a hydrophobic cavity composed of six conserved residues (Vannini et al., 2002; Zhang et al., 2002). Single-mutation analysis of some of these residues does not render AHL-binding incompetent TraR, but elevated signal concentrations—5000 to 10,000-fold– are then needed to achieve oxo-C8-HSL binding (Koch et al., 2005).

Additionally, it has been demonstrated that in X. oryzae pv. oryzae (Xoo), the LuxR solo OryR—which presents different critical amino acids in the AHL-binding domain– recognizes plant signals rather than AHLs (Ferluga et al., 2007; Ferluga and Venturi, 2009; González et al., 2013). Taking into account this observations and considering the variation in the AHL-binding domain of SmoR, it has been suggested that S. maltophilia SmoR might also recognize plant signals (Crossman et al., 2008), a possibility that has not been yet validated. We show here that SmoR binds AHLs, in particular the signal oxo-C8-HSL (Figure 2).

Genomic organization and sequence analysis have shown that oryR and xccR are not orthologous to smoR. Indeed, SmoR belongs to a recently classified subfamily designated “LuxR-like regulators chaperone HchA associated” as predicted by InterPro (http://www.ebi.ac.uk/interpro/) (Mitchell et al., 2014). Curiously, most bacteria sharing this particular operon display AHL production. However, there has been no functional study on the hchA-smoR operon. Nevertheless, the high homology observed between S. maltophilia HchA and E. coli Hsp31 suggests that, apart from being orthologous genes, both HchA and Hsp31 may regulate similar functions. In the genome of E. coli, the hchA gene is monocistronic. Its gene product Hsp31 has been widely studied in E. coli and its diverse functions have been elucidated. Initially, Hsp31 was reported to be a heat-inducible chaperone, showing feeble protease activity (Sastry et al., 2002; Malki et al., 2003, 2005). Further, it was shown that Hsp31 participates in heat shock and starvation response (Mujacic et al., 2004; Mujacic and Baneyx, 2006) as well as resistance to acid environments, generated during the stationary phase of growth (Mujacic and Baneyx, 2007). Recently it has been demonstrated that Hsp31 is a glyoxalase that participates in the detoxification of dicarbonyl stress (Subedi et al., 2011), which spans even more the functional spectrum of this versatile protein. Overall, this protein appears to act in front of stress environments derived from high cell density, a situation where QS systems are also active. In this line, we have shown that in S. maltophilia also a high cell density induces the expression of the hchA-smoR operon (Figure 3B). This suggests that S. maltophilia HchA may also act in front of stress situations such as starvation or accumulation of secondary metabolites, as described for E. coli Hsp31 (Mujacic and Baneyx, 2006, 2007; Subedi et al., 2011). In addition, we have observed that mutation of smoR results in a higher activity of operon during growth, which suggests that SmoR may act as a repressor in this situation (Figure 3B). On the other hand, we have observed in the wild type background that the presence of the exogenous signal C8-HSL significantly enhance in vivo promoter activity (Figure 3C). Although no systematic binding was observed for C8-HSL in the AHL-binding assay (data not shown), ß-galactosidase experiments make us reconsider whether SmoR could also bind to this signal, apart from oxo-C8-HSL. A possible explanation could rely on the use of different systems in each technique (note that AHL-binding assay was done in E. coli, while ß-galactosidase experiments have been performed in S. maltophilia). Therefore, further studies will be necessary to better understand the role of both eight-carbon AHL in the SmoR-dependent regulation. Interestingly, we have observed that the LuxR solos QscR (PA1898) from P. aeruginosa and the SmoR are putative orthologs. A new in vivo mechanism for LuxR activation depending on the free and signal-bond state has been proposed for QscR (Oinuma and Greenberg, 2011). It has been reported that although QscR binding to the signal 3-oxo-C6-HSL has a slightly effect on its own transcription (Lee et al., 2006), it can stimulate dimerization and activation, while preventing it from proteolysis (Oinuma and Greenberg, 2011; Chugani and Greenberg, 2014). A similar mechanism have been described for TraR regulator, suggesting that this new mechanisms might be widespread among LuxR homologs (Zhu and Winans, 1999, 2001), perhaps including SmoR. Altogether, we hypothesize that the regulator SmoR might bind to the palindromic box and block operon expression, until the presence of signal molecules bind to SmoR and avoid operon repression. Curiously, a highly related palindromic box was also identified between genes smlt2137 (universal stress family protein) and smlt2138 (transcriptional regulator nfxB) (Mitchell et al., 2014), two proteins that appear to be also involved in stress response. Nevertheless, determining whether SmoR could play an activator or a repressor role as well as which other genes could be under its regulation is something that will require further studies. Overall, our results suggest that in S. maltophilia, the hchA-smoR operon could have two important functions: (i) detoxification and recycling of secondary metabolites (HchA) and (ii) response to QS signals (SmoR), both deriving from situations of high cell density.

Interactions within microbial populations are common and essential for community maintenance (Ryan and Dow, 2008). In vitro studies of microbial consortia represent a first approach to uncover the complex interaction networks that occur between organisms in nature. Interspecific communication between S. maltophilia and P. aeruginosa has been a subject of investigation in the last years, since these two bacterial species usually share ecological niches and, importantly, they are frequently co-isolated in lungs of cystic fibrosis (CF) patients (Moskowitz et al., 2005). It has been reported that the DSF signal produced by S. maltophilia modulates P. aeruginosa behavior, including biofilm development and polymixin tolerance (Ryan et al., 2008) as well as virulence and persistence in lungs of CF patients (Twomey et al., 2012). However, as far as we know, the communication between these two potential human pathogens has been only studied in a unidirectional-way. We report here for the first time that S. maltophilia can also respond to signaling molecules produced by P. aeruginosa. In particular, we have shown that AHLs produced by P. aeruginosa stimulate swarming motility in S. maltophilia (Figure 4), a process in which SmoR might play a central role (Figure 5). Nevertheless, we cannot exclude that some other molecules present in the P. aeruginosa supernatant, such as rhamnolipids (Caiazza et al., 2005), could also participate in swarming stimulation. If so, it would explain the slightly stimulation observed in the ΔsmoR mutant, which perhaps could initiate its swarming motility due to the presence of rhamnolipids rather than AHL signals.

It is well established that complex population behaviors such as swarming motility are commonly regulated by AHL-QS systems (Daniels et al., 2004). Furthermore, previous studies have demonstrated that heterologous expression of lactonase AiiA from B. subtilis (Dong et al., 2000) reduces AHLs production and swarming motility in P. aeruginosa (Reimmann et al., 2002) and Burkholderia cepacia species (Wopperer et al., 2006). Regulation of bacterial motility by LuxR solos has been also reported. In Xoo, OryR positively regulates swimming and swarming motility by binding to the promoter of numerous flagella genes in response to plant signaling molecules (González et al., 2013).

To date, the only QS system described in S. maltophilia is DSF-QS, which is based on the signaling fatty acid molecule 11-cis-2-decenoic acid (Huang and Lee Wong, 2007; Huedo et al., 2014). Previous studies have evidenced that the DSF system regulates several virulence-related processes including bacterial motility, biofilm formation, antibiotic resistance and virulence (Fouhy et al., 2007; Deng et al., 2011; Huedo et al., 2014). In the related bacterium Burkholderia cenocepacia, both QS systems co-exist: the DSF –designated BDSF– (Boon et al., 2008; Deng et al., 2010) and the AHL (Wopperer et al., 2006) systems. Interestingly, it has been shown that certain biological functions such as motility, biofilm formation and virulence, are co-regulated by the BDSF- and AHL-dependent QS systems in B. cenocepacia (Deng et al., 2009, 2013). Although AHL production has not been reported in S. maltophilia, our findings suggest that, besides DSF, exogenous AHL signals could also regulate QS-related phenotypes—as observed for swarming motility–, by interacting with the LuxR solo SmoR.

Conflict of interest statement

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Supplementary material

The Supplementary Material for this article can be found online at: http://journal.frontiersin.org/article/10.3389/fcimb.2015.00041