ORIGINAL RESEARCH article
LbDSF, the Lysobacter brunescens Quorum-Sensing System Diffusible Signaling Factor, Regulates Anti- Xanthomonas XSAC Biosynthesis, Colony Morphology, and Surface Motility
- 1Institute of Plant Protection, Jiangsu Academy of Agricultural Sciences, Jiangsu Key Laboratory for Food Quality and Safety-State Key Laboratory Cultivation Base of Ministry of Science and Technology, Nanjing, China
- 2School of Life Sciences, Nantong University, Nantong, China
- 3Institute of Life Sciences, Jiangsu University, Zhenjiang, China
Lysobacter species are emerging as novel sources of antibiotics, but the regulation of these antibiotics has not been thoroughly elucidated to date. In this work, we identified a small diffusible signaling factor (DSF) molecule (LbDSF) that regulates the biosynthesis of a novel Xanthomonas-specific antibiotic compound (XSAC) in Lysobacter brunescens OH23. LbDSF was isolated from the culture broth of L. brunescens OH23, and the chemical structure of the molecule was determined by NMR and MS. The LbDSF compound induced GUS expression in a reporter strain of Xanthomonas campestris pv. campestris FE58, which contained the gus gene under the control of a DSF-inducible engXCA promoter. LbDSF production was found to be linked to the enoyl-CoA hydratase RpfF and dependent on the two-component regulatory system RpfC (hybrid sensor histidine kinase)/RpfG (response regulator), and LbDSF production was increased 6.72 times in the ΔrpfC compared to wild-type OH23. LbDSF-regulated XSAC production was dramatically decreased in ΔrpfF, ΔrpfC, and ΔrpfG. Additionally, a significant reduction in surface motility and a number of changes in colony morphology was observed in the ΔrpfF, ΔrpfC, and ΔrpfG compared to the wild-type OH23. The exogenous LbDSF significantly increased XSAC production in wild-type OH23 and recovered the XSAC biosynthetic ability in ΔrpfF. Taken together, these results showed that LbDSF is a fatty-acid-derived DSF that positively regulates XSAC biosynthesis, cell morphology, and surface motility. Moreover, the RpfC/RpfG quorum-sensing signal transduction pathway mediates XSAC biosynthesis. These findings may facilitate antibiotic production through genetic engineering in Lysobacter spp.
The gliding Gram-negative Lysobacter bacteria are ubiquitous freshwater and soil microorganisms; because they are fast-growing, simple to maintain, and genetically amenable for bioengineering, they are a promising source of novel bioactive natural antibiotics (Christensen and Cook, 1978; Xie et al., 2012). Some Lysobacter species have been demonstrated to be capable of producing antibiotics, including cyclodepsipeptides, cyclic lipodepsipeptides, cephem-type β-lactams, polycyclic tetramate macrolactams, phenazines, and lactivicins, which can inhibit the growth of plant pathogens.
Lysobactin is a cyclodepsipeptide that was first reported by O’Sullivan et al. (1988). The structure of lysobactin contains five natural amino acid residues and six non-proteinogenic amino acids, forming a macrocycle. Conversely, two families of cyclic lipodepsipeptides have been isolated from Lysobacter species (Kato et al., 1997; Hashizume et al., 2001; Zhang et al., 2011), both of which contain a β-hydroxyl fatty acid linked to the peptide moiety. The WAP-8294A family consists of 12 amino acid macrocycles, whereas the tripopeptin family is formed by eight amino acid cycles and a branched acyl group varying in length from 11 to 16 carbons (Xie et al., 2012). Cephem-type β-lactam antibiotics include cephalosporins, cephabacins, and cephamycins, but only cephabacins have been isolated from Lysobacter species (Harada et al., 1984; Ono et al., 1984). Cephabacins contain a cephem nucleus, which is linked to a non-ribosomal peptide by an ester linkage. Three different polycyclic tetramate macrolactams, xanthobacin, dihydromaltophilin (HSAF), and maltophilin, have been isolated from Lysobacter gummosus OH17 and Lysobacter enzymogenes OH11. All three of these polycyclic tetramate macrolactams contain γ-butyrolactam, which is involved in the macrocyclic structure (Meyers et al., 1985; Lou et al., 2011; Qian et al., 2013; Wang et al., 2013). Lysobacter cephabacins were shown to employ a novel mode of antibacterial action. These cephabacins specifically interfere with the biosynthesis of sphingolipids by targeting ceramide synthase, which causes thickening of the cell wall due to the accumulation of sphingolipid promoters that increase the degradation of chitin and block the elongation of the hyphal tips (Li et al., 2009). Several phenazines, including myxin and iodinin, have been found in Lysobacter antibioticus OH13 (Zhao et al., 2016). These phenazines differ not only in the presence of an N-oxide bond but also in the substituent at position 1 of the heterocycle. Finally, it is worth mentioning that lactivicin has a unique structure composed of a cycloserine ring linked to a γ-lactone ring (Harada et al., 1986). HSAF was shown to have a wide range of biological activities, including antibiotic, antifungal, and anticancer activities. Our research group also described a new cyclic lipodepsipeptide, WAP-8294A2, from L. enzymogenes, which exhibits strong inhibitory activity against methicillin-resistant Staphylococcus aureus (Zhang et al., 2011). WAP-8294A2 is currently in phase I/II clinical studies. WAP-8294A2 is produced by a large non-ribosomal peptide synthetase complex of 12 modules, which forms the linear assembly of amino acids. The biosynthetic pathway leading to the formation of 6 bioactive phenazines in L. antibioticus, starting from chorismic acid, was also reported by our research group (Zhao et al., 2016). After isolation of the compounds using reverse-phase HPLC, it was demonstrated that these phenazines exhibited strong activity against several bacteria, including Escherichia coli, Bacillus subtilis, and Xanthomonas spp.
In some prokaryotic systems, bacteria produce exogenous chemical signaling molecules to monitor population density and regulate a wide range of biological functions, such as secondary metabolite biosynthesis, biofilm formation, colony morphology, surface motility, and virulence (Abisado et al., 2018). LuxI/LuxR-type quorum-sensing systems are very common in Gram-negative bacteria, where they regulate the expression of genes through small chemical auto-inducers (Van Houdt et al., 2007). LuxI proteins are responsible for the synthesis of N-acyl homoserine lactone (AHL) quorum-sensing signals, and LuxR proteins are considered to be the main regulatory component of AHL quorum-sensing systems. These two proteins share two conserved regions, an AHL-binding domain and a DNA-binding domain (Maddocks and Oyston, 2008). Another group of quorum-sensing signals, the diffusible signaling factor (DSF) family, has recently been reported in a range of plant and human bacterial pathogens, including Xanthomonas campestris pv. campestris (Xcc), Xylella fastidiosa, Stenotrophomonas maltophilia, and L. enzymogenes (Barber et al., 1997; Deng et al., 2011; Robert and Dow, 2011; Han et al., 2015). In the DSF system, the putative enoyl-CoA hydratase RpfF is responsible for the synthesis of the DSF, and the RpfC/RpfG two-component system is involved in sensing and transducing DSF signals through a conserved phosphorelay mechanism (Holly et al., 2000). Different types of DSF signal molecules have been identified by electrospray ionization mass spectrometry (ESI-MS), gas chromatography, and nuclear magnetic resonance (NMR) analysis, such as cis-11-methyl-2-dodecenoic acid (DSF), cis-dodecenoic acid (BDSF), cis-11-methyldodeca-2,5-dienoic acid (CDSF), and 13-methyltetradecanoic acid (Wang et al., 2004; He et al., 2010; Han et al., 2015). Functional analysis of rpfF and rpfC mutants in different bacterial species suggests that the general role of the DSF-signaling system in virulence modulation is conserved, but the regulatory mechanisms and DSF-dependent traits may differ among taxa (Holly et al., 2000).
In this study, we isolated a novel Lysobacter brunescens strain, OH23, and active compounds from the culture supernatant of OH23 were shown to have strong specific activity against Xanthomonas species, whereas other bacteria and fungi, including Pseudomonas syringae pv. glycinea, P. syringae pv. lachrymans, Acidovorax citrulli, E. coli, Erwinia amylovora, Botryosphaeria dothidea, Phytophthora capsica, Valsa ambiens var. Pyri, and Colletotrichum gloeosporioide, remained unaltered (Supplementary Figure S1). We found that the genome of L. brunescens OH23 contained gene homologs to the regulation of pathogenicity factor (rpf) gene clusters of quorum-sensing genes from L. enzymogenes OH11. DSF signaling has been shown to be involved in the synthesis of metabolites with high pharmaceutical interest in L. enzymogenes OH11. This finding prompted us to investigate whether a DSF-dependent quorum-sensing signaling pathway was also responsible for the production of Xanthomonas-specific antibiotic compounds (XSAC). To this end, we developed single in-frame mutants of the homolog DSF genes rpfF, rpfC, and rpfG and tested their ability to both produce DSF signals and synthesize XSAC. Our results revealed that L. brunescens uses an autoregulatory mechanism similar to L. enzymogenes to control DSF biosynthesis, suggesting the production of a DSF-like molecule in L. brunescens (Holly et al., 2000). We characterized the L. brunescens DSF signal as 13-methyltetradecanoic acid and demonstrated that this molecule regulates XSAC biosynthesis, surface motility, and cell morphology through the RpfC/RpfG signaling pathway.
Materials and Methods
Bacterial Strains, Vectors, and Culture Conditions
The bacterial strains and plasmids used in this study are listed in Table 1. E. coli DH5α λpir, K-12, and S17-1 λpir were grown in LB (10 g tryptone, 5 g yeast extract, and 10 g sodium chloride, pH 7.0–7.2, in 1 L of distilled water) at 37°C (Sambrook, 2001). L. brunescens OH23 (stored at China General Microbiological Culture Collection Center, Beijing, CGMCC No. 13677) and the genetically engineered ΔrpfF, ΔrpfC, and ΔrpfG mutants were grown in nutrient broth (NB) medium (5 g peptone, 1 g yeast extract, 3 g beef extract, and 10 g sucrose, pH 7.0–7.2, in 1 L of distilled water) or in nutrient broth–yeast extract–glucose (NYG) medium (5 g peptone, 3 g yeast extract, and 20 g glycerol, pH 7.0–7.2, in 1 L of distilled water) at 28°C (Atlas, 1997). X. campestris pv. campestris FE58, Xanthomonas oryzae pv. oryzae PXO99A, X. oryzae pv. oryzae RS105, X. oryzae pv. oryzae KACC10331, X. campestris pv. campestris 8004, Xanthomonas axonopodis pv. glycines 12-2, P. syringae pv. glycinea PG4180, A. citrulli DSM17060, P. syringae pv. lachrymans 814/98, and E. amylovora ATCC15580 were also grown in nutrient broth (NB) medium at 28°C. All solid media contained 1.5% agar, and antibiotics were added at the following concentrations: 20 μg/ml rifampicin and 8 μg/ml gentamicin for L. brunescens, 50 μg/ml rifampicin, and 10 μg/ml tetracycline for X. campestris pv. campestris FE58, and 20 μg/ml gentamicin for E. coli. Sucrose was added at a final concentration of 4% for the counter-selection of in-frame deletion strains.
Generation of In-Frame Deletion Mutants
In-frame deletion plasmids were constructed by amplifying the flanking regions of specific genes by polymerase chain reaction (PCR) using Tks Gflex DNA Polymerase (TaKaRa Bio Inc., Kusatsu, Japan) and OH23 genomic DNA as the template according to the manufacturer’s instructions. Briefly, PCR amplification was performed using 30 PCR cycles consisting of denaturation at 98°C for 10 s, annealing at 55°C for 15 s, and elongation at 68°C for 1 min on a Bio-Red S1000 thermal cycler. The suicide vector pJQ200SK was digested with XbaI and BamHI (Thermo Fisher Scientific), and the target PCR fragments were ligated into the suicide vector using In-Fusion HD Cloning Plus (TaKaRa Bio Inc.). The recombinant vectors were transformed into E. coli DH5αλpir and confirmed using the universal primers M13F/M13R. The resulting plasmids were introduced into L. brunescens by conjugation. The deletion mutants ΔrpfF, ΔrpfC, and ΔrpfG were selected for double homologous recombination events because the suicide vector contained a sacB counter-selectable marker (Quandt and Hynes, 1993). Finally, all mutants were confirmed by PCR using specific primers (Table 2).
Lysobacter brunescens OH23 and the rpf mutants were cultured in NB medium at 28°C with shaking at 180 rpm until the OD600 was approximately 1.0 [which corresponds to approximately 109 CFU/ml (Colony Forming Units/ml)]. Then, 1 ml of culture for each strain was transferred into 50 ml of new liquid NB medium. The cultures were then incubated at 28°C with shaking at 180 rpm. To measure the growth, the OD600 value was determined every 12 h for each culture using a BioPhotometer Plus (Eppendorf, Germany) until each culture reached stationary stage. Three replicates were performed for each treatment, and the experiment was repeated three times.
Bioassay for DSF Activities in a DSF Reporter Strain
The fermentation and isolation of LbDSF was assessed as previously described (Han et al., 2015). After extracting the DSF-dependent quorum-sensing signals in L. brunescens OH23, we performed a DSF bioassay, as described previously with modifications (Wang et al., 2004). Briefly, L. brunescens OH23 and the ΔrpfF, ΔrpfC, and ΔrpfG mutants were grown in NB liquid medium (25 L liquid medium in a CRJ-50D fermenter, twice, for a total of 50 L) at 28°C at 180 rpm until the culture reached 2 × 109 CFU/ml (OD600 = approximately 2.0). The culture broth was centrifuged at 12,000 rpm for 10 min, and the supernatant was extracted with the same volume of ethyl acetate. The extracted organic phase was evaporated at 47°C, and the dry crude extract was partitioned using methanol and petroleum ether (100 ml each, three times). The petroleum ether phase was evaporated at 47°C, and the resulting oil (2.1 g) was dissolved in 10 ml of dimethyl sulfoxide (DMSO). The DSF-reporter strain, Xcc FE58, was grown in liquid NYG medium (5.0 g peptone, 3.0 g yeast extract, 20.0 g glycerol, and 1.0 L water, pH 7.2) for 2 days until the culture reached 3 × 109 CFU/ml (OD600 = approximately 3.0).
The bioassay plates were prepared using the following steps. First, 0.8 g agarose powder was added to 100 ml 0.5 × NYG liquid medium. The medium was heated until the agarose was resolved, at which point 60 μl of X-gluc (60 mg/ml) and 2 ml of the reporter strain Xcc FE58 culture (3 × 109 CFU/ml) were added into the NYG agarose medium (the medium was cooled to 42°C before use). This medium was used to prepare the 90-mm bioassay plates. Then, 5 μl of the DSF crude extract (10 mg crude extract resuspended in 200 μl of DMSO) from L. brunescens OH23, ΔrpfF, ΔrpfC, or ΔrpfG mutants was added to each well. The bioassay plates were incubated at 28°C for 24 h. The quantification of LbDSF was assessed as previously described (Wang et al., 2004). In brief, DSF activity was confirmed by the presence of a blue halo around the well and measured using the formula DSF (unit/ml) = 0.134 × e (1.9919W), where W is the diameter of the blue halo zone and the width of the blue halo zone was increased while adding more exogenous LbDSF (Figure 2B).
One unit of DSF is equivalent to a 1-cm-diameter blue halo zone formed by the addition of 0.18 ± 0.07 μg exogenous LbDSF. We also added DMSO to the bioassay plate as a negative control. Three replicates were performed for each treatment, and the experiment was repeated three times.
Isolation and Identification of LbDSF
The crude DSF extract was purified using HPLC. The HPLC detection conditions were as follows: reverse-phase HPLC (Shimadzu MS-2020, Tokyo, Japan) at 210 nm using a C-18 column (250 × 4.6 mm, Phenomenex). The mobile phase was 80% methanol in H2O from 0 to 13 min, 100% methanol in H2O from 13 to 20 min, and 80% methanol in H2O from 20 to 30 min (H2O containing 0.04% trifluoroacetic acid). The fraction corresponding to LbDSF appeared at 11.5 min.
Fractions containing the desired compound were evaporated to dryness under reduced pressure. The purified compound (4.3 mg) was dissolved in chloroform and characterized by mass spectrometry and NMR. High-resolution ESI-MS of the purified compound was performed in an AB (QTRAP 6500) instrument. The samples were directly infused into a mass spectrometer and analyzed in negative ion mode using a Turbo Ion Spray source. The NMR spectra (1H NMR and 13C NMR) were recorded in CD3OD using an AVANCE 600 (Bruker Company, Germany) instrument with a standard pulse program.
1H NMR (600 MHz, CDCl3): δ 2.35 (t, 2H, J = 7.8 Hz), 1.63 (qt, 2H, J = 7.2 Hz), 1.51 (sept, 1 H, J = 6.6 Hz), 1.37–1.24 (m, 16 H), 1.15 (m, 2 H), and 0.86 (d, 6 H, J = 6.6 Hz).
13C NMR (150 MHz, CDCl3): 179.97, 39.05, 34.01, 29.93, 29.69, 29.63, 29.59, 29.42, 29.23, 29.05, 27.97, 27.41, 24.67, and 22.65.
MS (ESI): calculated for C15H29O2 [M-H]− 241.2173, found 241.2.
Effect of the DSF-Dependent Quorum-Sensing System on XSAC Production
The ability of the wild-type and DSF mutants to produce XSAC was measured by an anti-Xanthomonas activity assay (diameter of inhibition zone) and analyzed using the agar diffusion method as described below. Pathogenic strains of Xanthomonas, including X. oryzae pv. oryzae PXO99A, X. oryzae pv. oryzae RS105, X. oryzae pv. oryzae KACC10331, X. campestris pv. campestris 8004, and X. axonopodis pv. glycines 12-2, were individually incubated in NB liquid medium until the culture OD600 was approximately 1.0. L. brunescens OH23, and its derived mutants (ΔrpfF, ΔrpfC, and ΔrpfG mutants) were incubated in NB liquid medium or NB liquid medium supplemented with 2 μM LbDSF until approximately 1.5–2.0 × 109 CFU/ml (OD600 = approximately 1.5–2.0). The cultures of L. brunescens OH23, ΔrpfF, ΔrpfC, and ΔrpfG were centrifuged, and the supernatants were incubated at 85°C for 30 min. For each pathogenic strain of Xanthomonas (Table 1 and Supplementary Table S1), 100 ml of liquefied NB solid medium was incubated at 45°C for 30 min, mixed with 108 cells, and then poured into plates. Then, 30 μl of supernatant from the cultures was spotted onto the selective plates. All plates were cultured at 28°C, and the zones of inhibition on the plates were photographed and compared after 2 days. XSAC production was confirmed by the diameter of the inhibition zone, and all of the data regarding the inhibition zone were subtracted from the diameter of the oxford cup. Three replicates were performed for each treatment, and the experiment was repeated three times.
Pathogenicity Assays in vivo
Oryza sativa ssp. indica rice cultivars IR24 and X. oryzae pv. oryzae PXO99A were used in the pathogenicity assay. O. sativa ssp. indica rice cultivars IR24 were grown under a 12-h light/dark cycle at 25°C with approximately 70% relative humidity for 2 months. The preparation of the supernatants from cultures of L. brunescens OH23, ΔrpfF, ΔrpfC, and ΔrpfG is described above. The leaves of IR24 plants were detached and dipped in the liquid culture of X. oryzae pv. oryzae PXO99A at a concentration of approximately 0.5 × 109 CFU/ml (OD600 = approximately 0.5) for 1 h. To determine the XSAC production and activity of wild-type OH23, ΔrpfF, ΔrpfC, and ΔrpfG, and chemically complemented strains, X. oryzae pv. oryzae PXO99A-infected rice leaves were treated with the respective supernatants every 24 h. For the negative control, X. oryzae pv. oryzae PXO99A-infected rice leaves were treated with NB medium. IR24 plants were grown in a glasshouse with the same conditions as above, and lesion lengths were measured and photographed at 7 dpi. Three replicates were performed for each treatment, and the experiment was repeated three times.
Detection and Comparison of Colony Morphology in L. brunescens
Single colonies of wild-type OH23, ΔrpfF, ΔrpfC, and ΔrpfG strains were inoculated on NYG plates or NYG plates containing 5 μM LbDSF for 3 days at 28°C. Then, the colony morphology of each strain was photographed and compared. Three replicates were used for each treatment, and the experiment was repeated three times.
Observation of Surface Motility
The surface motility assay of L. brunescens wild-type OH23, ΔrpfF, ΔrpfC, and ΔrpfG strains was performed as previously described (Song et al., 2017). Briefly, NB semi-solid medium containing 0.3% agar was used for surface motility assays, and 2.5 μl of L. brunescens wild-type OH23 or the derived mutants (109 CFU/ml, OD600 was approximately 1.0 for all strains) was spotted onto the surface of NB semi-solid medium plates or NB semi-solid medium plates containing 5 μM LbDSF. The plates were incubated at 28°C for 4 days, and then the surface motility of each strain was photographed, measured, and compared. Three replicates were performed for each treatment, and the experiment was repeated three times.
RNA Extraction, Reverse Transcription PCR, and Real-Time-PCR
Lysobacter brunescens OH23, ΔrpfF, ΔrpfC, and ΔrpfG mutants were each grown in 5 ml of NA medium to an OD600 of approximately 1.0. Three milliliters of cells was transferred into a sterile centrifuge tube and centrifuged for 3 min at 12,000 rpm. RNA was extracted from the strains using TRIzol solution (TaKaRa Biocompany) following the manufacturer’s instructions. For DNA removal and reverse transcription PCR, the PrimerScript RT Reagent Kit with the gDNA Eraser Kit (TaKaRa Biocompany) was used in this study. For the real-time PCR assay, a QuantStudio 6 Flex Real-Time PCR System (Thermo Fisher Scientific) was used to detect gene expression. The gene expression was calculated by the 2−ΔΔCT method. The primers for real-time PCR are listed in Supplementary Table S2. Three replicates were performed for each treatment, and the experiment was repeated three times.
Statistical analyses were calculated using SPSS (Statistical Package, Version 21.0). The variables were subjected to Student’s t-test and tested for significance at P < 0.05 (∗), P < 0.01 (∗∗), P < 0.001 (∗∗∗), and P < 0.0001 (∗∗∗∗).
Results and Discussion
Identification of the Small Signaling Molecule LbDSF in L. brunescens
To identify the structure of the DSF signal in L. brunescens OH23, we harvested the L. brunescens culture from a 50-L fermenter system (CRJ-50D), collecting 25 L each time for a total of 50 L, and we extracted the crude DSF from the supernatant using the same method as previously described (Han et al., 2015). The methods of separation and identification of the DSF from OH23 were described previously (Wang et al., 2004). Briefly, we collected samples every 2 min from HPLC, concentrated every fraction by evaporation, and added 1 μg of every sample into the DSF bioassay plates containing Xcc FE58 and X-gluc. The formation of a blue halo in the plates indicated the induction ability of each fraction. The results showed that the samples from 10.01 to 12.00 min induced gusA expression (Figures 1A,B). The DSF activity from 10.01 to 12.00 min was 0.53 ± 0.20 units. Furthermore, PengXCA-gusA was minimally induced by the addition of the samples from 0.01–10.00 or 12.01–16.00 min, and blue halo zones were not observed. To further confirm these results, we purified 1 μg of compound from these four fractions and detected the induction abilities of each fraction using the DSF bioassay system. The results of this assay revealed that PengXCA-gusA activation was induced only by adding the purified compound from fraction c, which exhibited a DSF activity of 1.98 ± 0.69 units.
Figure 1. Structural determination of the DSF from L. brunescens OH23. (A) HPLC analysis of the L. brunescens crude supernatant. (B) Bioassay of the four purified HPLC fractions a, b, c, and d from 10 to 12 min. The blue halo indicates DSF activity. (C) Mass spectrometry analysis of LeDSF3 (calculated [M-H]− = 241.2173 Da, observed 241.2 Da).
We also examined whether the compound from these fractions enhanced the anti-Xanthomonas activity in L. brunescens OH23. We collected, dried, and dissolved every fraction in DMSO. The supernatant from strain OH23 formed a zone of inhibition in the growth of X. oryzae pv. oryzae RS105 that was 2.15 ± 0.09 cm in diameter. The zone of inhibition increased to 2.77 ± 0.12 cm after the addition of 2.0 μM purified fraction c (Supplementary Figure S3). Moreover, the zone of inhibition did not significantly increase when the purified compounds from fraction a, fraction b, fraction d, or the DMSO control were added (Supplementary Figure S3). These results demonstrated that only the compounds from fraction c, collected at 11.5 min, enhanced the inhibition activities in strain OH23 (Supplementary Figure S3).
To identify the structure of the unidentified DSF compounds, we first collected approximately 2.6 mg of the compounds exhibiting the highest DSF activity (fraction c, 11.5 min) from 50 L of crude supernatant and resuspended it in chloroform for NMR analysis. After purification of the compounds from fraction c, mass spectrometry analysis of the purified compound revealed a main m/z fraction at 241.2 Da, which was consistent with the expected molecular weight of LeDSF3, [M-H]− = 241.2173 Da (Figure 1C). In contrast with most DSFs, the structure of LeDSF3 consisted of a saturated aliphatic chain, which was formed by a tetradecanoic acid structure with a methyl group linked to carbon 13. To confirm the presence of LeDSF3, 1H and 13C NMR spectra were collected, and all signals were assigned (Supplementary Figures S2A,B). In agreement with the expected structure, no signal was detected between 7 and 5 ppm in the 1H NMR spectrum, indicating that the purified compound was not an unsaturated aliphatic chain. A doublet with a 6.6-Hz coupling constant appeared at 0.86 ppm in the 1H NMR spectrum, corresponding to the methyl groups. The protons in the alpha and beta position to the carboxylic acid were observed at 2.35 and 1.63 ppm as a triple and a quintuplet, respectively, whereas the proton of carbon 13 appeared at 1.51 ppm as a septuplet. 13C NMR revealed a signal at 179.97 ppm, corresponding to the carboxylic acid. Carbon 2 was detected at 34.01 ppm, whereas the methyl groups appeared at 22.65 ppm in the 13C NMR spectrum. In agreement with the 1H NMR spectrum, no signal was detected between 180 and 120 ppm in the 13C NMR spectrum, discarding the possibility of an unsaturated chain. Therefore, the primary compound from fraction c, named LbDSF, was determined to be 13-methyltetradecanoic acid (Figure 1C), which was originally reported in L. enzymogenes (Han et al., 2015).
Identification of the rpf Gene Cluster in L. brunescens
As mentioned above, DSF family signals have been reported in different Xanthomonas bacteria. As a result, we compared and sequenced the genome of OH23 to identify genes potentially related to the LbDSF biosynthesis pathway. By blasting all rpf operon protein sequences1, we found that rpf proteins were highly conserved in Lysobacter spp. NCBI BLASTp analysis revealed that the Rpf proteins from L. brunescens had the highest homology to those of L. enzymogenes (taxid: 69), and the levels of protein identity were 72% (rpfF), 61% (rpfC), and 89% (rpfG). According to our BLASTp results, RpfF is an enoyl-CoA hydratase involved in the biosynthesis of DSF (Figure 2A). Accordingly, the DSF activity by wild-type OH23 was 0.88 ± 0.28 units, and the mutation of the rpfF gene abolished DSF production in L. brunescens (Figure 2B). RpfC is the hybrid histidine sensor kinase of the Rpf two-component regulatory system, which negatively regulates DSF production. Therefore, DSF accumulated in the ΔrpfC mutant (Figures 2A,B), and DSF production of ΔrpfC was 5.91 ± 2.29 units. RpfG is the response regulator of the Rpf two-component regulatory system and is responsible for signal transduction. Compared to wild-type OH23, DSF production was not altered in the ΔrpfG mutant (Figures 2A,B), and the DSF activity of the ΔrpfG was 0.63 ± 0.14 units.
Figure 2. Location of the rpf genes in the genome of L. brunescens OH23 and the DSF activity of the different L. brunescens OH23, rpf mutants, or L. enzymogenes OH11. (A) BLASTp comparison between the proteins encoded by the rpf genes (rpfF, rpfC, and rpfG) of L. brunescens and L. enzymogenes. The protein similarity was compared using BioEdit220.127.116.11. (B) The DSF production ability of strain OH23 and its corresponding rpf mutants. (C) The growth of wild-type OH23 and its corresponding rpf mutants.
Mutation of rpfF abolished the ability to produce DSFs in X. campestris pv campestris, which suggested that rpfF were essential for DSF production (Deng et al., 2011). In X. oryzae pv oryzae, the DSF production increased in the mutant of rpfC, and the DSF sensor kinase RpfC negatively regulated the biosynthesis of DSF (He et al., 2010; Deng et al., 2011). Taken together, these results indicate that the model for DSF production and signal transduction in L. brunescens is highly similar to that of L. enzymogenes and X. oryzae pv oryzae (He et al., 2010; Qian et al., 2013). In addition, the growth of wild-type OH23 and the rpf mutants was measured. The results demonstrated that the rpf mutants had growth similar to that of the wild-type strain under the tested conditions (Figure 2C).
DSF-Dependent Quorum-Sensing System Positively Regulates Antibiotic Biosynthesis Through the Small Signaling Molecule LbDSF and the RpfC/RpfG Two-Component System
In previous findings, the genus Xanthomonas and several Gram-negative bacteria used the DSF-dependent quorum-sensing system to mediate a diverse range of physiological activities related to virulence, motility, biofilm, and extracellular enzyme, and the DSF-dependent quorum-sensing system was also required for the biosynthesis of HSAF in L. enzymogenes (Qian et al., 2013; Guo et al., 2019). To investigate the function of the DSF-dependent quorum-sensing system in the biosynthesis of XSAC, we tested the anti-Xanthomonas abilities of the OH23 wild-type, ΔrpfF,ΔrpfG, ΔrpfC, and chemically complemented strains (mutants supplemented with LbDSF). As shown in Figures 3A,B and Supplementary Figures S4–S7, wild-type OH23 inhibited the growth of X. oryzae pv. oryzae PXO99A (Xoo PXO99A), X. oryzae pv. oryzae RS105 (Xoo RS105), X. oryzae pv. oryzae KACC 10331 (Xoo KACC 10331), X. campestris pv. campestris 8004 (Xcc 8004), and X. axonopodis pv. glycines 12-2 (Xag 12-2). The diameters of the inhibition zones were 1.22 ± 0.10 cm, 1.75 ± 0.15 cm, 1.95 ± 0.24 cm, 0.29 ± 0.09 cm, and 1.50 ± 0.14 cm, respectively. The ΔrpfF,ΔrpfG, and ΔrpfC mutants lost the ability to inhibit all tested Xanthomonas strains, demonstrating that these mutants were impaired in the biosynthesis of XSAC (Figure 3A and Supplementary Figures S4–S7). To determine the genes relevant to the XSAC biosynthesis, we analyzed the putative operon that related to the biosynthesis of XSAC (data not shown), and 8 genes of 13 genes were indispensable for the biosynthesis of XSAC (Supplementary Figures S8A,B). Furthermore, the q-PCR results shown that the expression of all 13 genes, the genes for XSAC biosynthesis, were dramatically reduced in the ΔrpfF mutant (Supplementary Figure S8C).
Figure 3. Anti-Xanthomonas activity of L. brunescens OH23 and its corresponding rpf mutants with or without LbDSF addition. (A) Supernatants from L. brunescens OH23 or rpf mutant cultures with or without exogenous LbDSF supplementation were tested for their antimicrobial activity against X. oryzae pv. oryzae PXO99A. (B) The analysis of the images of X. oryzae pv. oryzae PXO99A growth inhibition zones shown in A. (C) Representative images of IR24 leaves infected with X. oryzae pv. oryzae PXO99A and treated with test supernatants. CK is the control, which was treated with water every 24 h. Images were taken 7 days post-inoculation (dpi). (D) Analysis of the lesion lengths on IR24 rice leaves caused by X. oryzae pv. oryzae PXO99A infection with or without treatment with test supernatants, as shown in C. Different numbers of star (∗) above the bars indicate a significant difference between the wild-type strain OH23 and mutant strains (ns: not sigificant, ∗∗∗P < 0.001; ∗∗∗∗P < 0.001, t-test).
In L. enzymogenes, HSAF biosynthesis gene pks-nrps expression was reduced ∼10 times, and HSAF production was also dramatically reduced in the ΔrpfFOH11 mutant (Qian et al., 2013). Taken together, the DSF quorum-sensing XSAC biosynthesis regulation model in L. brunescens OH23 was similar to the DSF quorum-sensing HSAF biosynthesis regulation model in L. enzymogenes OH11, and the DSF quorum-sensing system positively regulated the biosynthesis of XSAC (Qian et al., 2013; Han et al., 2015).
To further address whether the small signaling molecule LbDSF restored XSAC biosynthesis in the rpf mutants, we added LbDSF (2 μM) to the mutant culture in liquid NB medium, incubated the culture at 28°C at 180 rpm, and then tested the anti-Xanthomonas activity of the supernatant. When LbDSF was added into the cultures, the growth inhibitory ability of wild-type OH23 increased 35.01, 19.54, 8.97, 16.86, and 27.15% against Xoo PXO99A, Xoo RS105, Xoo KACC 10331, Xcc 8004, and Xag 12-2, respectively (Figure 3A and Supplementary Figures S4–S7). LbDSF addition restored the anti-Xanthomonas activity in the ΔrpfF, and the diameter of the zones of inhibition were 0.84 ± 0.22 cm, 1.71 ± 0.16 cm, 0.36 ± 0.10 cm, 0.25 ± 0.11 cm, and 1.18 ± 0.16 cm against Xoo PXO99A, Xoo RS105, Xoo KACC 10331, Xcc 8004, and Xag 12-2, respectively (Figure 3A and Supplementary Figures S4–S7). Additionally, exogenous LbDSF had no effect on the anti-Xanthomonas activity in ΔrpfC and ΔrpfG (Figure 3A). These results were consistent with the fact that the small signaling molecule LbDSF is a transduction signal in the L. brunescens rpf system, where RpfF is involved in DSF biosynthesis, and RpfC/RpfG is the two-component system involved in signal transduction.
We then investigated whether all of the supernatants mentioned above had inhibitory activities in vivo. Xoo PXO99A-infected IR24 rice leaves were treated with the supernatants every 24 h, and lesion lengths were measured at 7 dpi. As shown in Figures 3C,D, the negative control was only treated with NB medium, and the lesion length was 2.92 ± 0.41 cm. However, the wild-type OH23 treatment group showed significantly decreased lesion lengths (0.70 ± 0.21 cm). The addition of exogenous LbDSF or DMSO to the culture of wild-type OH23 was shown to significantly influence the lesion length relative to the negative control. For the ΔrpfF treatment group, exogenous LbDSF restored the anti-Xanthomonas activity, and the lesion length was 0.83 ± 0.23 cm. However, both the ΔrpfG and ΔrpfC treatment groups exhibited similar lesion lengths as the negative control. The results from the in vivo plant assays were consistent with the results from the anti-Xanthomonas ability on plates.
In L. enzymogenes, LeDSF3 was 13-methyltetradecanoic acid, and acted as an extracellular signal to positively regulate the biosynthesis of HSAF; the two-component regulatory system RpfC/RpfG sensed and transduced LeDSF3; and the global regulator Clp was downstream of the LeDSF quorum-sensing system and also played a positive role in regulating the biosynthesis of HSAF and WAP-8294A2 (Han et al., 2015; Xu et al., 2016). To further investigate the function of clp in L. brunescens OH23, the ClpOH11 amino acid sequence was compared with the draft genome sequence of L. brunescens OH23, and Peg.2300 (Clp) shared 83% similarity to that of ClpOH11 at the amino acid level (Supplementary Figure S9A). Next, the anti-Xanthomonas abilities of Δclp and its complementary strain were tested, and clp had no significant effect on biosynthesis of XSAC (Supplementary Figure S9B), which revealed that Clp was not involved in the regulation of XSAC biosynthesis. Taken together, these findings indicate that the structure of LbDSF and the regulation of RpfC/RpfG L. brunescens were similar to the LeDSF quorum-sensing HSAF biosynthesis regulation model in L. enzymogenes and a potential novel transcription regulator in the DSF-dependent quorum-sensing system that regulated XSAC biosynthesis in L. brunescens.
DSF-Dependent Quorum-Sensing System Affects Colony Morphology in L. brunescens
The DSF quorum-sensing system was shown to influence colony morphology in L. enzymogenes (Qian et al., 2013). To investigate the function of the DSF-dependent quorum-sensing system in modulating colony morphology in L. brunescens, we tested the wild-type OH23 strain and the ΔrpfF, ΔrpfC, and ΔrpfG mutants. As shown in Figure 4, the wild-type OH23 displayed round colonies with lobular and spiculated boundaries on NYG plates with an average diameter size of 1.87 ± 0.05 cm. However, the ΔrpfF, ΔrpfC, and ΔrpfG mutants showed smooth colony appearance with an average diameter size of 0.64 ± 0.08 cm under the same growth conditions.
Figure 4. Colony morphology of wild-type OH23 and the rpf mutants on NYG plates with or without the exogenous addition of LbDSF. Each strain was grown in NYG liquid medium until the OD600 was approximately 1.0. Then, 3 μl of each strain was inoculated onto the surface of NYG plates. The plates were incubated at 28°C for 4 days. For the LbDSF treatment group, the strains were grown in NYG liquid medium containing 2 μM LbDSF, and the NYG plates contained 5 μM LbDSF. Each treatment was completed in triplicate, and the experiment was repeated three times.
Exogenous LbDSF (2 μM) restored the colony morphology in the ΔrpfF when compared to the wild-type OH23 with an average diameter size of 1.32 ± 0.08 cm, whereas the addition of exogenous LbDSF did not influence the colony morphology of the ΔrpfC and ΔrpfG (Figure 4). These results indicate that the DSF-dependent quorum-sensing system is involved in the regulation of colony morphology in L. brunescens.
DSF Signaling Controls Surface Motility Through Type IV Pili (T4P) in L. brunescens
The DSF-dependent quorum-sensing system was also shown to affect cell motility in L. enzymogenes (Qian et al., 2013). To investigate the function of the DSF-dependent quorum-sensing system in regulating motility in L. brunescens, we tested the motility of the wild-type OH23, ΔrpfF, ΔrpfC, and ΔrpfG strains. Since OH23, unlike L. enzymogenes OH11, does not exhibit twitching motility (data not shown), we analyzed the surface motility of wild-type OH23 and its derivative mutants on NB semi-solid (0.3% agar) motility medium plates for 4 days incubated at 28°C.
As shown in Figure 5A, the wild-type OH23 strain was motile in motility medium plates with a typical circular dissemination pattern from the point of inoculation that was 2.78 ± 0.33 cm in size. However, the surface motility of ΔrpfF, ΔrpfC, or ΔrpfG was substantially reduced. These mutants only reached an average surface motility diameter of approximately 0.82 ± 0.11 cm in 4 days, indicating that the mutants had a 73.72% reduction in the diameter of their surface motility zone compared to the wild-type OH23. Exogenous LbDSF (2 μM) restored surface motility in the ΔrpfF strain compared to the wild-type OH23 strain with an average surface motility diameter of 2.42 ± 0.10 cm. However, exogenous LbDSF did not exhibit any effect on the surface motility in the ΔrpfC and ΔrpfG mutants. These results indicate that the DSF-dependent quorum-sensing system is involved in the regulation of surface motility in L. brunescens.
Figure 5. Surface motility of wild-type OH23 and the rpf mutants with or without the exogenous addition of LbDSF. (A) Surface motility of wild-type OH23 and the rpf mutants with or without the exogenous addition of LbDSF. Each strain was grown in liquid NB medium until the culture reached an OD600 of approximately 1.0. Then, 3 μl of strain was inoculated onto the surface of NB plates. The plates were inoculated at 28°C for 4 days. For the LbDSF treatment group, the strains were grown in NYG liquid medium containing 2 μM LbDSF. (B) pilA1 expression in wild-type OH23 and the rpf mutants with or without the exogenous addition of LbDSF. Different numbers of star (∗) above the bars indicate a significant difference between the wild-type strain OH23 and mutant strains (ns: not sigificant, ∗∗∗P < 0.001; ∗∗∗∗P < 0.001, t-test).
Type IV Pili has been shown to be important for surface motility in diverse bacteria. Since the pilA gene encodes the major pilin subunit of T4P (Mattick, 2002; Burdman et al., 2011; Wang et al., 2014), we measured pilA1 expression in the wild-type OH23, ΔrpfF, ΔrpfC, and ΔrpfG. As shown in Figure 5B, pilA1 expression was dramatically decreased in ΔrpfF, ΔrpfC, and ΔrpfG. The addition of exogenous LbDSF (2 μM) partially restored pilA1 expression in the ΔrpfF compared to wild-type OH23, while exogenous LbDSF did not influence pilA1 expression in the ΔrpfC and ΔrpfG. These results indicate that the DSF-dependent quorum-sensing system is involved in the regulation of pilA1 expression in L. brunescens.
The DSF-dependent quorum-sensing system in the Xanthomonas genus differs substantially between species and has been shown to positively regulate virulence, biofilm formation, EPS biosynthesis, and adaption. Moreover, specific DSF molecules were related to specific antibiotic HSAF biosynthesis (He et al., 2010; Han et al., 2015). The Rpf system was shown to be activated by adding specific DSF molecules, and EPS production, extracellular xylanase activity, or antibiotic HSAF biosynthesis were restored (He et al., 2010; Han et al., 2015).
In this study, we report the role of a quorum-sensing system in the production of a novel XSAC in the ubiquitous environmental bacterium L. brunescens (Figure 6). Our data revealed that L. brunescens OH23 uses a DSF-dependent quorum-sensing molecule to regulate XSAC production. We characterized this DSF compound as 13-methyltetradecanoic acid. This extracellular signal is produced by RpfF and transduced by the RpfC/RpfG two-component regulatory system. This molecule also regulates surface motility and colony morphology. Our findings will be useful in applied genetics and molecular biotechnology, thereby facilitating the improvement of antibiotic production in Lysobacter spp., which can potentially be used in the agricultural industry. Furthermore, the tight control that our identified DSF molecule exerts on XSAC expression suggests that Lysobacter spp. may produce other quorum-sensing signals that can induce the production of additional novel bioactive compounds.
Figure 6. Schematic model of the DSF quorum-sensing system in L. brunescens. LbDSF biosynthesis was found to be linked to RpfF (enoyl-CoA hydratase) and was dependent on the two-component regulatory system RpfC (hybrid sensor histidine kinase)/RpfG (response regulator). LbDSF positively regulates XSAC biosynthesis, surface motility, and cell morphology.
The datasets generated for this study can be found in Genbank, MK532476, MK532477, and MK532478.
JL, RZ, PL, TJ, YJ, and YZ conducted the experiments. FL designed and conducted the experiments. JL, PL, and FL contributed to the writing of the manuscript. FL revised the manuscript.
This study was supported by the Jiangsu Agricultural Science and Technology Innovation Funds [CX (16) 1049], the Jiangsu Provincial Key Technology Support Programme (BE2015354), the “948” Project of the Ministry of Agriculture (2014-Z24), the Earmarked Fund for China Agriculture Research System (CARS-28-16), and the China Postdoctoral Science Foundation (2017M610310).
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.
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fmicb.2019.01230/full#supplementary-material
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Keywords: diffusible signaling factor, anti-Xanthomonas compound, colony morphology, surface motility, Lysobacter brunescens
Citation: Ling J, Zhu R, Laborda P, Jiang T, Jia Y, Zhao Y and Liu F (2019) LbDSF, the Lysobacter brunescens Quorum-Sensing System Diffusible Signaling Factor, Regulates Anti- Xanthomonas XSAC Biosynthesis, Colony Morphology, and Surface Motility. Front. Microbiol. 10:1230. doi: 10.3389/fmicb.2019.01230
Received: 14 February 2019; Accepted: 17 May 2019;
Published: 18 June 2019.
Edited by:Cristina García-Aljaro, University of Barcelona, Spain
Reviewed by:Meriyem Aktas, Ruhr-Universität Bochum, Germany
Shaohua Chen, South China Agricultural University, China
Copyright © 2019 Ling, Zhu, Laborda, Jiang, Jia, Zhao and Liu. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Fengquan Liu, email@example.com
†These authors have contributed equally to this work