Skip to main content
Download PDF

RpfC regulates the expression of the key regulator hrpX of the hrp/T3SS system in Xanthomonas campestris pv. campestris

BMC Microbiology volume 18, Article number: 103 (2018) Cite this article

Abstract

Background

The Gram-negative phytopathogenic bacterium Xanthomonas campestris pv. campestris recruits the hrp/T3SS system to inject pathogenicity effector proteins into host cells and uses the rpf/DSF cell-cell signaling system to regulate the expression of virulence factors such as extracellular enzymes and polysaccharide. Whether these two systems have any connection is unknown.

Methods

Positive regulator candidates affecting hrpX expression were identified by sacB strategy. The transcriptional expression was determined by qRT-PCR and GUS activity analysis. Transcriptome analysis was performed by RNA deep-sequencing. The hypersensitive response (HR) was determined in the nonhost plant pepper ECW-10R and electrolyte leakage assay.

Results

Mutation of the gene encoding the sensor RpfC of the rpf/DSF system significantly reduced the expression of hrpX, the key regulator of the hrp/T3SS system, all of the genes in the hrp cluster and most reported type III effector genes. Mutation of rpfG did not affect the expression of hrpX. The rpfC mutant showed a delayed and weakened HR induction.

Conclusions

RpfC positively regulates the expression of hrpX independent of RpfG, showing a complex regulatory network linking the rpf/DSF and hrp/T3SS systems.

Background

The Gram-negative bacterium Xanthomonas campestris pathovar campestris (Xcc) is the causal agent of black rot disease, one of the most destructive diseases of cruciferous crops worldwide [1]. This pathogen can infect almost all members of the crucifer family (Brassicaceae), including many important vegetables, the major oil crop rape, and the model plant Arabidopsis thaliana. Over the past several decades, Xcc has been used as a model bacterium for studying molecular mechanisms of bacterial pathogenicity [2]. The entire genome sequences of a number of strains such as ATCC33913, 8004, and B100 have been determined [3,4,5] and a large number of genes associated with essential virulence have been identified. Among them, rpf (regulation of pathogenicity factors) and hrp (hypersensitive response and pathogenicity) clusters of genes are essential for pathogenicity of Xcc [6,7,8].

The Xcc rpf cluster of genes consists of at least nine genes (rpfA to rpfI). This gene cluster is involved in the quorum sensing system, controlling the synthesis of a diffusible signal factor (DSF) and regulating extracellular plant cell wall-degrading enzymes and extracellular polysaccharide (EPS) production as well as biofilm formation [6, 9,10,11]. The role of rpfC, rpfF and rpfG genes has been extensively studied [9,10,11,12,13,14,15,16,17]. The rpfF gene encodes an enzyme responsible for synthesizing the DSF molecules, which are secreted into extracellular environment [16]. The proteins encoded by rpfC and rpfG compose a two-component signal transduction system which is implicated in DSF perception and signal transduction [9, 12, 13]. RpfC acts as the histidine kinase sensor in the two component regulatory system to sense the environmental DSF signal, leading to activation of RpfG as a cyclic di-GMP phosphodiesterase. The activation of RpfG then leads to a reduction of cyclic di-GMP level which promotes synthesis of extracellular enzymes and EPS [9, 12, 13]. In addition, it is known that cyclic di-GMP effects on the synthesis of extracellular enzymes and EPS involve the transcriptional activator Clp (cAMP receptor-like protein). Cyclic di-GMP binds to Clp, thus preventing binding of Clp to the promoters of target genes that include those encoding extracellular enzymes and EPS biosynthesis [13,14,15,16,17].

In addition to the rpf/DSF regulatory system, the pathogenicity of Xcc is also dependent on the hrp cluster of genes. The hrp genes are associated with pathogen-induced hypersensitive response (HR), a disease-resistant phenomenon at the infection sites of resistant hosts and nonhost plants, and pathogen’s pathogenicity in susceptible hosts. Most hrp genes in the cluster encode the type III secretion system (T3SS) that translocates effector proteins into host cells and is highly conserved among Gram-negative pathogenic bacteria [18,14,20]. In Xcc, the hrp cluster is composed of six main operons (hrpA to hrpF) which harbor more than 20 different genes [7]. The expression of the operons is regulated by the AraC-type transcriptional activator HrpX [21]. The expression of hrpX is positively regulated by a two-component signal transduction system composed of HpaS and HrpG [21, 22]. HpaS is a histidine kinase sensor and HrpG is an OmpR family response regulator [22]. It is clear that the expression of the hrp genes including the regulators hrpG and hrpX is expressed at low levels in nutrient rich media but induced in plant tissues or in certain minimal media [7, 21].

As the hrp genes are induced in minimal media but expressed at low levels in nutrient rich media, the studies on the hrp/T3SS system were commonly carried out in certain minimal media. On the contrary, the rpf/DSF system is studied in nutrient rich media. To our knowledge, no work on the link between rpf/DSF and hrp/T3SS systems has been reported. The aim of this work was to identify upstream regulators of hrpX in Xcc. We employed the sacB strategy [23] to screen mutations that affect the expression of hrpX. Interestingly, we found that a mutation in the rpfC gene of the rpf/DSF system significantly reduced the expression of hrpX. Here, we provide evidences showing that RpfC positively regulates hrpX.

Methods

Bacterial strains, plasmids and growth conditions

The bacterial strains and plasmids used in this work are listed in Table 1. Xcc strains were grown at 28 °C in nutrient rich medium NYG [24] or minimal media MMX (23.8 mM glucose, 3.87 mM sodium citrate, 15.1 mM (NH4)2SO4, 0.81 mM MgSO4, 23 mM K2HPO4, 44 mM KH2PO4, pH 7.0) [24] and XCM1 (20 mM succinic acid, 0.15 g/l casamino acids, 7.57 mM (NH4)2SO4, 1 mM MgSO4, 60.34 mM K2HPO4, 33.07 mM KH2PO4, pH 6.6) [25]. Antibiotics were used at the following final concentrations as required: ampicillin (Amp), 100 μg/ml; gentamycin (Gm), 10 μg/ml; kanamycin (Kan), 25 μg/ml; rifampicin (Rif), 50 μg/ml; and tetracycline (Tc), 15 μg/ml for Escherichia coli and 5 μg/ml for Xcc. E. coli strains were grown in Luria-Bertani medium (LB, per liter: tryptone 10 g, yeast extract 5 g, NaCl 10 g) at 37 °C. The triparental conjugation between Xcc and E. coli strains was performed as described by Daniels and associates [24]. Restriction enzymes and DNA ligase were used in accordance with the manufacturer’s instructions (Promega, Madison, Wisconsin, USA).

Table 1 Bacterial strains and plasmids used in this work
Full size table

Screen for mutations affecting the expression of hrpX

In order to screen the genes influencing the expression of hrpX, the sacB system [26] was employed. The 1419-bp sacB gene without the start codon ATG was amplified from the plasmid pK18mobsacB [27] (Table 1) using the primer pair sacB-F/sacB-R (Table 2). After confirmation by sequencing, the amplified sacB gene was ligated into the plasmid pLAFR6 [28] (Table 1), yielding the recombinant plasmid pL6sacB (Table 1). The promoter of hrpX was then in-frame cloned into pL6sacB, generating the plasmid pL6hrpXsacB, in which the sacB gene is driven by the hrpX promoter (Table 1). The plasmid pL6hrpXsacB was introduced into Xcc wild type strain 8004 from E. coli by triparental conjugation, yielding the strain 8004/pL6hrpXsacB (Table 1). The bacterial cells of strain 8004/pL6hrpXsacB were treated to be competent status and mutated by the EZ-Tn5™ transposon using a commercial EZ-Tn5™ transposon kit (Epicentre Biotechnology), followed by selecting mutant colonies on the plates of MMX minimal medium containing Rif, Kan, Tc and 5% sucrose.

Table 2 Primers used in this work
Full size table

To map the transposon insertion sites in the obtained mutants, the total DNA of each mutant was isolated and digested with EcoRI (no EcoRI site within the transposon), and then cloned into the plasmid pUC19 [29] (Table 1). The resulting recombinant plasmid was transformed into E. coli strain JM109 [29] (Table 1) and transformants were selected by Kan (for the transposon) plus Amp resistance. The recombinant plasmid was isolated from the obtained Kan- and Amp-resistant transformants and the DNA sequences flanking the transposon were identified by sequencing the recombinant plasmid using the primers KAN-2 FP-1 or KAN-2 RP-1 (Table 2).

Construction of mutants and GUS reporters

An rpfC deletion mutant was generated by the methods described previously [30]. Briefly, two DNA fragments flanking rpfC gene were generated by PCR using the primer pairs RpfC-1-FOR/RpfC-1-REV and RpfC-2-FOR/RpfC-2-REV (Table 2). The resultant DNA fragments were cleaved with BamHI and ligated. The fusion fragments were then amplified using the ligation mixture as the template and the primer pair RpfC-1-FOR/RpfC-2-REV and cloned into the SmaI site of vector pK18mobsacB and transformed into E. coli strain JM109. After sequence verification, the obtained recombinant plasmid was mobilized into Xcc strain 8004 by triparental conjugation. Transconjugants were firstly selected on NYG medium supplemented with Rif and Kan. The second selection was made on NYG medium containing 5% sucrose and Rif for resolution of the vector by a second crossover event. The in-frame deletion of rpfC was confirmed by PCR and sequencing.

To construct Xcc hrpG and hrpX promoter-gusA transcriptional fusion reporters, the promoter regions of hrpG and hrpX were amplified from Xcc strain 8004 using the primer sets PhrpG-F/PhrpG-R and PhrpX-F/PhrpX-R (Table 2), respectively. The amplified hrpG promoter fragment and hrpX promoter fragment were double digested with SacI plus XbaI and EcoRI plus KpnI, respectively, then ligated into the plasmid pUC19 (Table 1). The resulting recombinant plasmids were then transformed into E. coli JM109. Transformants were selected on LB medium supplemented with IPTG, X-gal (5-Bromo-4-chloro-3-indolyl-β-D-galactoside) and Kan. The positive colonies were confirmed by PCR and sequencing, generating the plasmids pUCPhrpG and pUCPhrpX (Table 1). The promoter regions of hrpG and hrpX were excised from plasmids pUCPhrpG and pUCPhrpX and cloned into pLGUS [31] (Table 1) and transformed into E. coli JM109. Transformants were selected on LB medium supplemented with Tc. Recombinant plasmids were isolated from the obtained transformants and confirmed by PCR and restriction enzyme digestion. The confirmed recombinant plasmids were named pGUShrpG and pGUShrpX, respectively. These reporter plasmids were subsequently transferred into Xcc strains ΔrpfC and 8004 by triparental conjugation. Transconjugants were selected on NYG medium supplemented with Rif and Tc. The resulting transconjugants 8004/pGUShrpG, ΔrpfC/pGUShrpG, 8004/pGUShrpX, and ΔrpfC/pGUShrpX (Table 1) were further confirmed by PCR and restriction enzyme digestion.

HR test and electrolyte leakage assay

HR test was performed as described previously [32]. The Xcc nonhost plant pepper ECW-10R (Capsicum annuum cv. ECW-10R) was used. Pepper seedlings were grown in a greenhouse with 12 h day and night cycle illumination by fluorescent lamps at temperatures of 25 to 28 °C. Bacterial cells of Xcc strains from overnight cultures were washed and diluted to a concentration at an optical density at 0.01 (600 nm) (1 × 107 CFU/ml) in 10 mM sodium phosphate buffer (5.8 mM Na2HPO4 and 4.2 mM NaH2PO4, pH 7.0) and approximately 5 μl bacterial suspension was infiltrated into the pepper leaf tissues at the stage of four fully expanded leaves using a needleless syringe. After infiltration, the plants were grown at 28 °C with a 16 h photoperiod per day and 80% relative humidity. HR symptoms were photographed at 8, 16, and 24 h post-inoculation. At least three plants were inoculated in each experiment, and each experiment was repeated at least three times.

For electrolyte leakage assay, bacterial suspensions were diluted to a concentration of OD600 = 0.01 in 10 mM sodium phosphate buffer and measurements were carried out exactly as described previously [33]. Essentially, for each sample, four leaf disks were removed with a 0.7-cm diameter cork borer, submerged in 10 ml of distilled water, and vacuum-infiltrated. Then, the net leakage after 1 h was measured with a conductivity meter (DDS-307A). Three samples were taken for each measurement in each experiment; the experiments were repeated at least twice.

GUS activity assay

Xcc cells from overnight culture in NYG medium were resuspended in XCM1 medium to a final optical density of 0.1 (600 nm) and incubated for 24 h. Then, 1 ml of the culture was transferred to another 10 ml fresh XCM1 medium and incubated for 24 h. To determine the β-glucuronidase (GUS) activity of the bacterial cells, 200 μl cultures for each strain were mixed with 40 μl methylbenzene and vortexed. The supernatant was then taken for GUS activity assay. The GUS activity assay was performed by measurement of the OD415 using ρ-nitrophenyl-β-D-glucuronide as substrate as described previously [34].

Histochemical GUS staining

Chinese radish cv. Manshenhong seedlings with four fully expanded leaves were used for inoculation. Histochemical GUS staining was performed by using 5-bromo-4-chloro-3-indolylglucuronide (Promega) as a substrate as described previously [34]. Bacterial suspensions of Xcc strains were diluted to a concentration of OD600 = 0.01 in sterile water and introduced into host plant leaves. For GUS activity quantification of bacterial cells in the plant leaves, the fluorogenic substrate 4-methylumbelliferyl-β-D-glucuronide was used following the method described previously [35]. For plant protein extraction, 10 mg plant leaves were added to 1 ml of cold GUS extraction buffer [50 mM Na3PO4, pH 7.0, 10 mM β-mercaptoethanol, 10 mM EDTA, 0.1% (w/v) sodium lauryl sarcosine, and 0.1% (w/v) Triton X-100] and grinded with mortar and pestle until homogenized. Then, 30 μl 0.1% SDS and 60 μl chloroform were added. After 10 s vortexes, samples were transformed into micro-centrifuge tubes and centrifugalized for 8 min at 8000 rcf. The plant extract protein was quantified and immediately tested by adding the GUS assay buffer [2 mM 4-MUG (4-Methyl-umbelliferyl-β-D-Glucuronide)]. The assay was performed using 5-bromo-4-chloro-3-indolylglucuronide (X-Gluc) (Promega) as substrate, essentially as described previously [35]. At least four wells for each concentration of MUG (two with plant extract and two with extraction buffer to serve as blanks and correct for any nonenzymatic hydrolysis of MUG). Final MUG concentrations of 10 μM, 30 μM, 50 μM, 70 μM, and 90 μM were used for plotting a standard curve. A 30 μM MUG was chosen to react with samples and the final volume was 100 μl. The plate was incubated at 37 °C for 10 min and then removed from heat and sat at room temperature for 2.5 h. Then, 200 μl of 0.2 M carbonate stop buffer was added to each well. Fluorescence was determined with emission and excitation filters set at 465 nm and 360 nm, respectively. The values for each time interval were averaged after subtracting the blank.

Transcriptome analysis

Xcc cells from overnight culture in NYG medium were collected, washed twice with MMX medium and then transferred to 10 ml fresh MMX medium to a final optical density of 0.3 (600 nm) and incubated till the concentration up to OD600 = 0.6. The total RNA was extracted from the cultures with SV Total RNA Isolation System (Promega). RNA samples were quantified and qualified by Agilent Bioanalyzer (Agilent Technologies). The RNA integrity number (RIN) of total RNA should be greater than 8.0 and the rRNA ratio (23S/16S) should be greater than 1.2. The total RNA samples were digested by RQ DNase I (Promega) with a concentration of 1 U/μg of RNA samples. The RNA samples for transcriptome analysis were prepared according to the manufacturer’s manuals (Illumina). Briefly, rRNA was cleaned by Ribo-Zero™ rRNA Removal Kit (Gram-Negative Bacteria) (Epicentre Biotechnologies). After purification, the mRNA was fragmented into small pieces for first strand cDNA synthesis using the fragment agent (divalent cations) under elevated temperature. The synthesized cDNA fragments were added with adapters at their ends by an end repair process. The obtained products were purified and enriched with PCR to create the final cDNA libraries. The quality of these cDNA libraries was assessed using the Agilent Bioanalyzer and ABI Step One Plus Real-Time PCR (Applied Biosystems). The RNAs were sequenced by the Illumina sequencing platform (HiSeq 2000) in Beijing Genomics Institute at Shenzhen (BGI).

Analysis of sequence data

The raw reads generated from the sequencing were cleaned up and mapped to the reference genomic sequence of Xcc strain 8004 by SOAP2/SOAP aligner [36]. The expression levels were evaluated by reads per kilobase per million mapped reads (RPKM) [37], which normalizes the reads count to the gene expression level by taking account of the gene length and sequencing depth. The differential expression genes (DEGs) analysis was performed as described by Audic and Clavier [38], in which false discovery rate (FDR) was used to determine the threshold of p-value in multiple tests. In this study FDR < 0.001 was used as the threshold to judge the significance of gene expression difference. RNA sequencing data from four samples [ΔrfpC-1, ΔrfpC-2, Xcc 8004–1 (WT-1), Xcc 8004–2 (WT-2)] were grouped into four pairs (ΔrfpC-1/WT-1, ΔrfpC-1/WT-2, ΔrfpC-2/WT-1, and ΔrfpC-2/WT-2). The log2 fold change of RPKM of mutant vs. wild type was counted. The average of the log2 fold values of the four pairs was used to assess the differential expression genes with a stringent cutoff value of |log2-fold value| ≥ 1.0 and p value < 0.01. The RNA sequencing strategy for ΔrpfG was the same as ΔrpfC.

qRT-PCR analysis

Xcc cells from overnight culture in NYG medium were collected, washed twice with MMX medium and transferred to 10 ml fresh MMX medium to a final optical density of 0.3 (600 nm) and incubated till the concentration up to OD600 = 0.6. The total RNA was extracted from the cultures with SV Total RNA Isolation System (Promega). The PrimeScriptTM RT reagent Kit with gDNA Eraser (Perfect Real Time) (TakaRa) was employed to fulfill the digestion of genomic DNA and the synthesis of cDNA. The obtained cDNA template was diluted to a final concentration of 5 ng/μl and 2 μl aliquot was used for qRT-PCR analysis. 16S rDNA gene was used for normalization in the qRT-PCR analysis. The primer sets for randomly selected ORFs, hrp genes, and type III effector genes were listed in Table 2.

Results

Identification of positive regulator candidates affecting hrpX expression by sacB strategy

The sacB gene that encodes a levansucrase in Bacillus subtilis has been used as a tool for positive selection [23, 39,40,41]. The enzyme levansucrase catalyzes transfructorylation from sucrose to various acceptors, resulting in sucrose hydrolysis and the synthesis of levan, which is toxic to cells. It has been reported that expression of sacB gene in the presence of 5% sucrose in agar medium is lethal to a variety of bacteria including E. coli, Agrobacterium tumefaciens, and Rhizobium meliloti [23]. In this study, we found that similar to these bacteria, Xcc strain 8004 expressing sacB gene could not survive at the same sucrose concentration. Therefore, we used the sacB gene to screen candidates which positively regulate the expression of hrpX. In brief, firstly we constructed a recombinant plasmid pL6hrpXsacB (Table 1) by cloning a sacB gene into the broad host range plasmid pLAFR6 (Table 1), in which the sacB gene was driven by the promoter of hrpX. Then, the plasmid pL6hrpXsacB was transferred from E. coli into Xcc wild type strain 8004 by triparental conjugation. The obtained transconjugant strain 8004/pL6hrpXsacB (Table 1) was mutated by the EZ-Tn5™ transposon, followed by selecting mutant colonies on the plates of MMX minimal medium containing 5% sucrose. The principle in this strategy is that strain 8004/pL6hrpXsacB cannot grow on the minimal medium MMX containing 5% sucrose (Fig. 1b), because the expression of the hrpX-promoter-driven sacB gene is lethal to the cells under these conditions. However, the strains with a mutation (i.e., deletion mutant of hrpG, ΔhrpG) impeding the expression of hrpX (i.e. strain ΔhrpG/pL6hrpXsacB) (Fig. 1c) or disrupting the sacB gene and the wild-type strain 8004 as well as the deletion mutant strain ΔhrpG can grow (Fig. 1a and d).

Fig. 1
figure 1

Identification of positive regulator candidates affecting hrpX expression by sacB strategy. Xcc wild type train 8004 and the deletion mutant strain ΔhrpG were used as controls. The principle in this strategy is that strain 8004/pL6hrpXsacB cannot grow on the minimal medium containing 5% sucrose, because the expression of the hrpX-promoter-driven sacB gene is lethal to the cells under these conditions, and only the strains with a mutation (i.e., deletion mutant of hrpG, ΔhrpG) impeding the expression of hrpX (i.e. strain ΔhrpG/pL6hrpXsacB, or disrupting the sacB gene, or the wild-type strain 8004 and the deletion mutant strain ΔhrpG can grow. a, wild-type strain 8004; b, 8004/pL6hrpXsacB; c, ΔhrpG/pL6hrpXsacB; d, the deletion mutant strain ΔhrpG

Full size image

Six mutants (named XB001 to XB006) (Table 1) were obtained in this work. The transposon insertion sites in these mutants were further mapped (see Methods for details), revealing that the mutations lie in the ORFs XC_4007 (XB001), XC_2333 (XB003), XC_1192 (XB004), XC_3951 (XB005) and XC_0124 (XB006), and the intergenetic region between the ORFs XC_1510 and XC_1511 (XB002), respectively. Interestingly, the ORF XC_2333 is the rpfC gene. The others were annotated to encode hypothetical proteins (XC_4007 and XC_1511), antifreeze glycopeptide AFGP related protein (XC_1192), glucosyltransferase (XC_3951), TonB-dependent receptor (XC_0124), and TldD protein (XC_1510), respectively.

RpfC positively regulates the expression of hrpX

As described above, RpfC is a key sensor kinase in rpf/DSF system. The above result suggests that RpfC may also play a role in the regulation of hrp/T3SS system. To further validate this result, we constructed a deletion mutant of rpfC (named ΔrpfC) and promoter-gusA transcriptional fusion reporter plasmids of Xcc hrpG and hrpX (named pGUShrpG and pGUShrpX) (see the Methods for details). The reporter plasmids were then transferred into the rpfC deletion mutant ΔrpfC and the wild-type strain 8004 by triparental conjugation, yielding reporter strains ΔrpfC/pGUShrpG, ΔrpfC/pGUShrpX, 8004/pGUShrpG, and 8004/pGUShrpX, respectively (Table 1). Subsequently, GUS activities of these strains grown in hrp-inducing minimal medium XCM1 were assayed. The results showed that the GUS activities of the strain ΔrpfC/pGUShrpX was significantly lower than that of the strain 8004/pGUShrpX (p = 0.005 by t test) (Fig. 2). Although the GUS activity of strain ΔrpfC/pGUShrpG was lower than that of strain 8004/pGUShrpG, their difference was not significant (P = 0.3344 by t test) (Fig. 2). These data suggest that RpfC is involved in positive regulation of the expression of hrpX and the regulation is probably independent of HrpG in the minimal medium XCM1.

Fig. 2
figure 2

RpfC positively affects the expression of hrpX in XCM1 minimal medium. β-Glucuronidase (GUS) activities of hrpG and hrpX promoter-gusA reporters in the rpfC mutant and the wild-type backgrounds. Strains were cultured in XCM1 medium for 24 h, and GUS activities were then determined by measurement of optical density at 415 nm (OD415) using ρ-nitrophenyl-β-D-glucuronide as substrate. Data are mean ± standard deviations (SD) of triplicate measurements. The experiment was repeated twice and similar results were obtained. **, t-test, p < 0.01

Full size image

To investigate whether RpfC regulates the expression of hrpG and hrpX in plants, the above reporter strains were inoculated into the host plant Chinese radish and the GUS activity in the inoculated levels were measured. As shown in Fig. 3, the strain ΔrpfC/pGUShrpX produced significantly lower GUS activity compared to the strain 8004/pGUShrpX, suggesting that RpfC positively regulates the expression of hrpX in planta. Interestingly, the strain ΔrpfC/pGUShrpG also produced significantly lower GUS activity compared to the strain 8004/pGUShrpG (Fig. 3). This indicates that RpfC regulates the expression of hrpG in planta. Taken together, these results imply that RpfC regulates the expression of hrpX in the minimal medium XCM1 as well as in the host plant Chinese radish and influences significantly the expression of hrpG in the host plant tissues but not in XCM1 medium.

Fig. 3
figure 3

RpfC positively affects the expression of hrpG and hrpX in host plant. Xcc strains 8004/pGUShrpG, 8004/pGUShrpX, ΔrpfC/pGUShrpG, and ΔrpfC/pGUShrpX were cultured in NYG medium overnight and resuspended in water to an optical density at 600 nm of 0.01, and then inoculated into the Chinese radish cv. Manshenhong leaves by leaf clipping. At 5 days post-inoculation, the inoculated leaves were assayed. a, Leaves were taken and analyzed for bacterial numbers and GUS activity was measured with the fluorogenic substrate 4-methylumbelliferyl-β-D-glucuronide. GUS activity values per 108 bacterial cells are the mean ± standard deviations of three independent measurements. b, GUS activity was measured using an in situ staining method, and bacterial cell numbers inside the infected leaves were measured in a parallel experiment. Average bacterial numbers inside the tested leaves are indicated. The experiments were repeated twice. Data presented are from a representative experiment, and similar results were obtained in the other independent experiment

Full size image

Mutation of rpfC results in a delayed and weakened HR induction

The above results showed clearly that rpfC positively regulates the expression of the key regulator hrpX of the hrp/T3SS system. To verify whether mutation of rpfC affects the pathogen to induce HR on plants, the mutant strain ΔrpfC and the complemented strain CΔrpfC (Table 1) were tested on Xcc nonhost pepper cultivar ECW-10R (Capsicum annuum cv. ECW-10R), which carries the resistance gene Bs1 and has been typically used to test the HR of Xcc [33]. The experiment was carried out by infiltrating bacterial suspensions with a cell concentration of OD600 = 0.01 into the plant leaves. Strain ΔavrBs1, an avrBs1-deletion mutant of Xcc, which cannot elicit any HR symptoms on the pepper cultivar [42], was included as a negative control. Eight hours after inoculation, no significant HR phenotype was observed for the mutant strain ΔrpfC, while typical HR symptoms induced by the wild type strain 8004 and the complemented strain CΔrpfC were observed (Fig. 4a). However, the mutant strain ΔrpfC produced visible HR symptoms 16 h after inoculation (Fig. 4a). These results were further substantiated using an electrolyte leakage assay. Both mutants (ΔrpfC and ΔavrBs1) showed significantly decreased electrolyte leakages at 8, 16, and 24 h after inoculation compared to the wild-type strain, although ΔrpfC showed stronger electrolyte leakage than ΔavrBs1 (Fig. 4b). Consistent with the HR symptoms observed, the complemented strain and the wild type induced similar electrolyte leakages 16 h after inoculation (Fig. 4b). Taken together, these results reveal that RpfC is important for Xcc to stimulate a full HR on the nonhost plant pepper cultivar ECW-10R.

Fig. 4
figure 4

RpfC is involved in hypersensitive response. a, Hypersensitive response symptoms induced in pepper leaves (Capsicum annuum cv. ECW-10R) by the Xcc strains. Approximately 5 μl bacterial culture (1 × 107 CFU/ml) suspended in 10 mM sodium phosphate buffer were infiltrated into the leaf mesophyll tissue with a blunt-end plastic syringe. Pictures of the pepper leaf were taken at 8, 16, and 24 h after infiltration. Three replications were done in each experiment, and each experiment was repeated three times. Results presented are from a representative experiment, and similar results were obtained in all other independent experiments. b, Electrolyte leakage from pepper leaves inoculated with Xcc strains. Results presented are from a representative experiment, and similar results were obtained in other independent experiments

Full size image

RpfC and RpfG regulate the expression of a large set of genes in Xcc 8004

To verify whether mutation of rpfC affects the expression of hrp genes via rpfG in minimal medium, the transcriptome of the mutant strains ΔrpfC and ΔrpfG were determined by RNA deep-sequencing. The mutant strains and the wild type strain 8004 were cultivated in the minimal medium MMX to a cell concentration of OD600 = 0.6–0.8. Total RNA was extracted from the cultures with SV Total RNA Isolation System (Promega). The RNA sequencing was carried out according to the manufacturer’s standard procedure (BGI). Through data analysis (Additional file 1: Table S1), a total of 528 RpfC-regulated genes were identified, among them 328 and 200 were down- and up-regulated, respectively; while 626 RpfG-regulated genes were identified, of which 283 and 343 were down- and up-regulated, respectively. Based on the published gene list of Xcc strain 8004 [4], the products of the RpfC- and RpfG-regulated genes could be grouped into the following 20 functional categories: (I) Nucleotide metabolism, (II) Carbohydrate metabolism, (III) Amino acid and protein metabolism, (IV) Chaperon and peptidases, (V) Fatty acid metabolism, (VI) Extracellular enzymes, (VII) Sugar kinase/transaminase, (VIII) Multidrug resistance and detoxification, (IX) Oxidative stress resistance, (X) Flagellum synthesis and motility, (XI) Hypersensitive reaction and pathogenicity, (XII) Iron uptake, (XIII) Ribosomal proteins, (XIV) Transcription regulators, (XV) Dehydrogenase, (XVI) Aerobic and anaerobic respiration, (XVII) Membrane components and transporters, (XVIII) Hypothetical proteins, (XIX) Environmental information processing, (XX) Others (Fig. 5, Additional file 2: Table S2 and Additional file 3: Table S3). To validate the transcriptome data, qRT-PCR was carried out. The result showed that the transcriptional expression of the 24 randomly selected genes, 2 hrp genes [hrpB1 (XC_3011) and hrpF (XC_3025)], and 2 type III effector genes (XC_0241 and XC_4273) was highly consistent with the transcriptome result (Fig. 6). A comparison of the genes regulated by RpfC and RpfG revealed that only 279 of them were regulated by both RpfC and RpfG (Fig. 5). This indicates that the regulons of RpfC and RpfG are not all the same.

Fig. 5
figure 5

Comparison of RpfC and RpfG regulons. Venn diagrams showing the overlap of genes (a, Total regulated genes. b, hrp genes. c, Type III effector genes) whose expression is upregulated or downregulated in rpfC or rpfG deletion mutant backgrounds

Full size image
Fig. 6
figure 6

qRT-PCR verification of differently expressed genes in ΔrpfC (a) and ΔrpfG (b). The genes were chosen randomly from the transcriptome results. Two independent experiments were performed, and similar results were obtained. Results presented are from a representative experiment

Full size image

RpfC positively regulates 25 hrp genes, 9 reported T3S effector genes

The transcriptome result displayed that the expression of all the genes in the hrp cluster (XC_3001-XC_3025) and the regulator hrpX in ΔrpfC mutant cells was significantly (p ≤ 0.01 by t-test) lower than that in the wild type strain (Table 3). Furthermore, in ΔrpfC mutant cells the expression of the 9 reported T3S effector genes (XC_0241, XC_1553, XC_2004, XC_2081, XC_2602, XC_2995, XC_3160, XC_3177, and XC_4273) was also significantly (P ≤ 0.01 by t-test) lower than that in the wild type [3, 31, 42,43,44] (Table 3). However, the expression of hrpG and the global regulator clp in rpf/DSF system was not affected by the mutation of rpfC in the tested conditions (Table 3).

Table 3 RpfC positively regulates the expression of hrpX, 25 hrp genes, and 9 T3S effectors
Full size table

Notably, the transcriptome analysis revealed that mutation of rpfG did not affect the expression of hrpG, hrpX and clp (Table 4), but significantly (P ≤ 0.01 by t test) influence the expression of some hrp genes (XC_3009 to XC_3015, XC_3019, XC_3021, and XC_3025) and most of the reported T3S effector genes (XC_0241, XC_2004, XC_2081, XC_2602, XC_2995, XC_3160, XC_3177, and XC_4273) (Table 4). Given that RpfC and RpfG compose a two-component regulatory system, it is worthy to further study how they regulate the hrp and T3S effector genes. Nevertheless, these results reveal that RpfC positively regulates the expression of hrp and T3S effector genes as well as hrpX but not hrpG and clp in the minimal medium MMX.

Table 4 RpfG positively regulates the expression of 10 hrp genes, 8 T3S effectors
Full size table

Discussion

The above results demonstrate that the sensor RpfC of the rpf/DSF cell-cell signaling system positively regulates the expression of the key regulator hrpX of the hrp/T3SS system in Xcc. Disruption of the rpfC gene in Xcc strain 8004 caused a significant decrease in the transcription of the hrp genes in minimal medium and host plant (Fig. 2, Fig. 3, Table 3, Table 4), resulting in a delayed and weakened HR (Fig. 4). The cell-cell signaling system is generally considered to facilitate gene expression when the bacterial population has reached a sufficient cell density [45]. Almost all of the previous studies on the rpf/DSF system of Xcc and its regulation in the synthesis of the virulence factors such as extracellular enzymes and EPS were carried out by growing bacterial cells in nutrient rich conditions to allow the bacterium to reach a high cell density. On the contrary, as the expression of hrp genes is repressed in nutrient rich media and induced in certain minimal media and plants, almost all of the studies on the hrp/T3SS system were carried out in minimal media or plants. The connection between these two systems has been neglected. We were lucky that rpfC gene was identified in the mutagenesis screen for hrpX-upstream regulatory genes.

Recent evidence suggests that perception of the DSF signal by RpfC leads to activation of RpfG as a phosphodiesterase that degrades cyclic di-GMP. Cyclic di-GMP is a second messenger which can bind to Clp to prevent binding of Clp to the promoters of target genes. The Clp regulator contains an N-terminal cNMP binding domain and a C-terminal DNA-binding domain. The decrease in cyclic di-GMP level by the phosphodiesterase activity relieves this inhibition, thus allowing Clp to bind to target promoter DNA sequences and activate target gene expression [13, 14, 46,47,48]. In a previous transcriptome profiling analysis in Xcc strain XC1 cultivated in a nutrient rich medium, it was found that mutation of clp affects the transcription of 299 genes. Within these Clp-regulated genes, 260 were up-regulated and 39 down-regulated. The latter genes include 9 hrp genes (hrpB5, hrpD5, hrcR, hrpW, hpaP, hrpB2, hrpB7, hrpB4, and hpa1) but neither hrpG nor hrpX [15]. These implied that RpfC regulates the expression of the hrp genes might via RpfG and the global transcriptional regulator Clp in Xcc. However, An and associates found that mutation of rpfC or rpfG in Xcc strain 8004 grown in the nutrient rich medium NYG did not affect the expression of hrp genes [49]. Our RNA sequencing data demonstrated that in minimal medium, RpfC positively regulates the expression of nearly all the hrp genes (Table 3) and RpfG controls some of the hrp genes (Table 4). These results indicate that RpfC and RpfG have different effects on the expression of the hrp genes in Xcc strain 8004 when grown in nutrient-rich and nutrient-deficient conditions. Our data also displayed that in minimal medium RpfC regulates the expression of hrpX but not hrpG and RpfG does not regulate the expression of both hrpG and hrpX (Table 3, Table 4). These results suggest that RpfC activate the expression of hrpX in minimal medium via neither RpfG nor HrpG. However, mutation of rpfC significantly reduced the expression of not only hrpX but also hrpG in planta (Fig. 3). This implies that RpfC regulates the hrp genes via different manners in minimal medium and host plants.

As mentioned above, it is known that the core regulatory mechanism in Xcc rpf/DSF quorum sensing system is RpfC-RpfG-c-di-GMP-Clp cascade. However, our transcriptome result showed that the regulons of RpfC and RpfG in the minimal medium MMX are not all the same. Similarly, the regulons of RpfC and RpfG of Xanthomonas citri subsp. citri in nutrient rich medium are also different [50]. These findings suggest that RpfC may regulate a number of genes independent of RpfG. Our data presented in this work show that RpfC may employ an undefined pathway other than the RpfC-RpfG-c-di-GMP-Clp cascade to regulate the expression of the hrp key regulator HprX in the minimal medium MMX. To further dissect how RpfC affects the expression of hrpX will be commendable. Interestingly, RpfC controls the expression of hrpG in host plants (Fig. 3). This suggests that the regulation net between the rpf/DSF and hrp/T3SS systems are rather complex. To further uncover this issue will be valuable.

Conclusions

In this work, we found that mutation of the gene encoding the sensor RpfC of the rpf/DSF system significantly reduced the expression of hrpX, the key regulator of the hrp/T3SS system. Here, we provide evidences to demonstrate that RpfC positively regulates the expression of hrpX independent of RpfG, the cognate response regulator of RpfC, showing a complex regulatory network linking the rpf/DSF and hrp/T3SS systems.

Abbreviations

4-MUG:

4-Methyl-umbelliferyl-β-D-Glucuronide

Amp:

Ampicillin

BGI:

Beijing Genomics Institute

CFU:

Colony forming unit

Clp:

cAMP receptor-like protein

DEGs:

Differential expression genes

DSF:

Diffusible signaling factor

FDR:

False discovery rate

Gm:

Gentamycin

GUS:

β-glucuronidase

HR:

Hypersensitive response

hrp :

Hypersensitive response and pathogenicity

Kan:

Kanamycin

Rif:

Rifampicin

rpf :

Regulation of pathogenicity factors

RPKM:

Reads per kilobase per million mapped reads

SD:

Standard deviations

T3SS:

Type III secretion system

Tc:

Tetracycline

Xcc :

Xanthomonas campestris pv. campestris

X-Gal:

5-Bromo-4-chloro-3-indolyl-β-D-galactoside

X-Gluc:

5-bromo-4-chloro-3-indolylglucuronide

References

  1. Vicente JG, Holub EB. Xanthomonas campestris pv. campestris (cause of black rot of crucifers) in the genomic era is still a worldwide threat to brassica crops. Mol Plant Pathol. 2013;14(1):2–18.

    Article  PubMed  CAS  Google Scholar 

  2. Mansfield J, Genin S, Magori S, Citovsky V, Sriariyanum M, Ronald P, et al. Top 10 plant pathogenic bacteria in molecular plant pathology. Mol Plant Pathol. 2012;13(6):614–29.

    Article  PubMed  Google Scholar 

  3. da Silva AC, Ferro JA, Reinach FC, Farah CS, Furlan LR, Quaggio RB, et al. Comparison of the genomes of two Xanthomonas pathogens with differing host specificities. Nature. 2002;417(6887):459–63.

    Article  PubMed  Google Scholar 

  4. Qian W, Jia Y, Ren SX, He YQ, Feng JX, Lu LF, et al. Comparative and functional genomic analyses of the pathogenicity of phytopathogen Xanthomonas campestris pv. campestris. Genome Res. 2005;15(6):757–67.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  5. Vorhölter FJ, Schneiker S, Goesmann A, Krause L, Bekel T, Kaiser O, et al. The genome of Xanthomonas campestris pv. campestris B100 and its use for the reconstruction of metabolic pathways involved in xanthan biosynthesis. J Biotechnol. 2008;134(1–2):33–45.

    Article  PubMed  CAS  Google Scholar 

  6. Tang JL, Liu YN, Barber CE, Dow JM, Wootton JC, Daniels MJ. Genetic and molecular analysis of a cluster of rpf genes involved in positive regulation of synthesis of extracellular enzymes and polysaccharide in Xanthomonas campestris pathovar campestris. Mol Gen Genet. 1991;226(3):409–17.

    Article  PubMed  CAS  Google Scholar 

  7. Arlat M, Gough CL, Barber CE, Boucher C, Daniels MJ. Xanthomonas campestris contains a cluster of hrp genes related to the larger hrp cluster of Pseudomonas solanacearum. Mol Plant-Microbe Interact. 1991;4(6):593–601.

    Article  PubMed  CAS  Google Scholar 

  8. Ryan RP, Vorholter FJ, Potnis N, Jones JB, Van Sluys MA, Bogdanove AJ, et al. Pathogenomics of Xanthomonas: understanding bacterium–plant interactions. Nat Rev Microbiol. 2011;9(5):344–55.

    Article  PubMed  CAS  Google Scholar 

  9. Barber CE, Tang JL, Feng JX, Pan MQ, Wilson TJ, Slater H, et al. A novel regulatory system required for pathogenicity of Xanthomonas campestris is mediated by a small diffusible signal molecule. Mol Microbiol. 1997;24(3):555–66.

    Article  PubMed  CAS  Google Scholar 

  10. Dow JM, Crossman L, Findlay K, He YQ, Feng JX, Tang JL. Biofilm dispersal in Xanthomonas campestris is controlled by cell-cell signaling and is required for full virulence to plants. Proc Natl Acad Sci U S A. 2003;100(19):10995–1000.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  11. Cai Z, Yuan ZH, Zhang H, Pan Y, Wu Y, Tian XQ, et al. Fatty acid DSF binds and allosterically activates histidine kinase RpfC of phytopathogenic bacterium Xanthomonas campestris pv. campestris to regulate quorum-sensing and virulence. PLoS Pathog. 2017;13(4):e1006304.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  12. Dow M. Diversification of the function of cell-to-cell signaling in regulation of virulence within plant pathogenic xanthomonads. Sci Signal. 2008;1(21):pe23.

    Article  PubMed  Google Scholar 

  13. Ryan RP, Dow JM. Communication with a growing family: diffusible signal factor (DSF) signaling in bacteria. Trends Microbiol. 2011;19(3):145–52.

    Article  PubMed  CAS  Google Scholar 

  14. Chin KH, Lee YC, Tu ZL, Chen CH, Tseng YH, Yang JM, et al. The cAMP receptor-like protein CLP is a novel c-di-GMP receptor linking cell-cell signaling to virulence gene expression in Xanthomonas campestris. J Mol Biol. 2010;396(3):646–62.

    Article  PubMed  CAS  Google Scholar 

  15. He YW, Ng AY, Xu M, Lin K, Wang LH, Dong YH, et al. Xanthomonas campestris cell-cell communication involves a putative nucleotide receptor protein Clp and a hierarchical signalling network. Mol Microbiol. 2007;64(2):281–92.

    Article  PubMed  CAS  Google Scholar 

  16. He YW, Zhang LH. Quorum sensing and virulence regulation in Xanthomonas campestris. FEMS Microbiol Rev. 2008;32(5):842–57.

    Article  PubMed  CAS  Google Scholar 

  17. Ryan RP, Fouhy Y, Lucey JF, Jiang BL, He YQ, Feng JX, et al. Cyclic di-GMP signalling in the virulence and environmental adaptation of Xanthomonas campestris. Mol Microbiol. 2007;63(2):429–42.

    Article  PubMed  CAS  Google Scholar 

  18. Alfano JR, Collmer A. Type III secretion system effector proteins: double agents in bacterial disease and plant defense. Annu Rev Phytopathol. 2004;42:385–414.

    Article  PubMed  CAS  Google Scholar 

  19. Cornelis GR, Van Gijsegem F. Assembly and function of type III secretory systems. Annu Rev Microbiol. 2000;54:735–74.

    Article  PubMed  CAS  Google Scholar 

  20. Jones JD, Dangl JL. The plant immune system. Nature. 2006;444(7117):323–9.

    Article  PubMed  CAS  Google Scholar 

  21. Huang DL, Tang DJ, Liao Q, Li XQ, He YQ, Feng JX, et al. The Zur of Xanthomonas campestris is involved in hypersensitive response and positively regulates the expression of the hrp cluster via hrpX but not hrpG. Mol Plant-Microbe Interact. 2009;22(3):321–9.

    Article  PubMed  CAS  Google Scholar 

  22. Li RF, Lu GT, Lei Li SHZ, Feng GF, Chen Y, et al. Identification of a putative cognate sensor kinase for the two-component response regulator HrpG, a key regulator controlling the expression of the hrp genes in Xanthomonas campestris pv. campestris. Environ Microbiol. 2014;16(7):2053–71.

    Article  PubMed  CAS  Google Scholar 

  23. Gay P, Le Coq D, Steinmetz M, Berkelman T, Kado CI. Positive selection procedure for entrapment of insertion sequence elements in gram-negative bacteria. J Bacteriol. 1985;164(2):918–21.

    PubMed  PubMed Central  CAS  Google Scholar 

  24. Daniels MJ, Barber CE, Turner PC, Cleary WG, Sawczyc MK. Isolation of mutants of Xanthomonas campestris pv. campestris. showing altered pathogenicity Microbiology. 1984;130(9):2447–55.

    Google Scholar 

  25. Jiang GF, Jiang BL, Yang M, Liu S, Liu J, Liang XX, et al. Establishment of an inducing medium for type III effector secretion in Xanthomonas campestris pv. campestris. Braz J Microbiol. 2014;44(3):945–52.

    Article  PubMed  PubMed Central  Google Scholar 

  26. Recorbet G, Robert C, Givaudan A, Kudla B, Normand P, Faurie G. Conditional suicide system of Escherichia coli released into soil that uses the Bacillus subtilis sacB gene. Appl Environ Microbiol. 1993;59(5):1361–6.

    PubMed  PubMed Central  CAS  Google Scholar 

  27. Schäfer A, Tauch A, Jäger W, Kalinowski J, Thierbach G, Pühler A. Small mobilizable multi-purpose cloning vectors derived from the Escherichia coli plasmids pK18 and pK19: selection of defined deletions in the chromosome of Corynebacterium glutamicum. Gene. 1994;145(1):69–73.

    Article  PubMed  Google Scholar 

  28. Huynh TV, Dahlbeck D, Staskawicz BJ. Bacterial blight of soybean: regulation of a pathogen gene determining host cultivar specificity. Science. 1989;245(4924):1374–7.

    Article  PubMed  CAS  Google Scholar 

  29. Yanisch-Perron C, Vieira J, Messing J. Improved M13 phage cloning vectors and host strains: nucleotide sequences of the M13mp18 and pUC19 vectors. Gene. 1985;33(1):103–19.

    Article  PubMed  CAS  Google Scholar 

  30. He YW, Wang C, Zhou L, Song H, Dow JM, Zhang LH. Dual signaling functions of the hybrid sensor kinase RpfC of Xanthomonas campestris involve either phosphorelay or receiver domain-protein interaction. J Biol Chem. 2006;281(44):33414–21.

    Article  PubMed  CAS  Google Scholar 

  31. Jiang BL, He YQ, Cen WJ, Wei HY, Jiang GF, Jiang W, et al. The type III secretion effector XopXccN of Xanthomonas campestris pv. campestris is required for full virulence. Res Microbiol. 2008;159(3):216–20.

    Article  PubMed  CAS  Google Scholar 

  32. An SQ, Lu GT, Su ZH, Li RF, He YQ, Jiang BL, Tang DJ, Tang JL. Systematic mutagenesis of all predicted gntR genes in Xanthomonas campestris pv. campestris reveals a GntR family transcriptional regulator controlling hypersensitive response and virulence. Mol Plant-Microbe Interact. 2011;24(9):1027–39.

    Article  PubMed  CAS  Google Scholar 

  33. Castañeda A, Reddy JD, El-Yacoubi B, Gabriel DW. Mutagenesis of all eight avr genes in Xanthomonas campestris pv. campestris had no detected effect on pathogenicity, but one avr gene affected race specificity. Mol Plant-Microbe Interact. 2005;18(12):1306–17.

    Article  PubMed  CAS  Google Scholar 

  34. Jefferson RA, Kavanagh TA. Bevan MW. GUS fusions: beta-glucuronidase as a sensitive and versatile gene fusion marker in higher plants. EMBO J. 1987;6(13):3901–7.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  35. Vojnov AA, Slater H, Daniels MJ, Dow JM. Expression of the gum operon directing xanthan biosynthesis in Xanthomonas campestris and its regulation in planta. Mol Plant-Microbe Interact. 2001;14(6):768–74.

    Article  PubMed  CAS  Google Scholar 

  36. Li H, Handsaker B, Wysoker A, Fennell T, Ruan J, Homer N, Marth G, et al. The sequence alignment/map format and SAMtools. Bioinformatics. 2009;25(16):2078–9.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  37. Mortazavi A, Williams BA, McCue K, Schaeffer L, Wold B. Mapping and quantifying mammalian transcriptomes by RNA-Seq. Nat Methods. 2008;5(7):621–8.

    Article  PubMed  CAS  Google Scholar 

  38. Audic S, Claverie JM. The significance of digital gene expression profiles. Genome Res. 1997;7(10):986–95.

    Article  PubMed  CAS  Google Scholar 

  39. Lepesant JA, Lepesant-Kejzlarova J, Pascal M, Kunst F, Billault A, Dedonder R. Identification of the structural gene of levansucrase in Bacillus subtilis Marburg. Mol Gen Genet. 1974;128(3):213–21.

    Article  PubMed  CAS  Google Scholar 

  40. Lawes M, Maloy S. MudSacI, a transposon with strong selectable and counterselectable markers: use for rapid mapping of chromosomal mutations in Salmonella typhimurium. J Bacteriol. 1995;177(5):1383–7.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  41. Pierce JC, Sauer B. Sternberg N. A positive selection vector for cloning high molecular weight DNA by the bacteriophage P1 system: improved cloning efficacy. Proc Natl Acad Sci U S A. 1992;89(6):2056–60.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  42. He YQ, Zhang L, Jiang BL, Zhang ZC, Xu RQ, Tang DJ, et al. Comparative and functional genomics reveals genetic diversity and determinants of host specificity among reference strains and a large collection of Chinese isolates of the phytopathogen Xanthomonas campestris pv. campestris. Genome Biol. 2007;8(10):R218.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  43. Jiang W, Jiang BL, Xu RQ, Huang JD, Wei HY, Jiang GF, et al. Identification of six type III effector genes with the PIP box in Xanthomonas campestris pv. campestris and five of them contribute individually to full pathogenicity. Mol Plant-Microbe Interact. 2009;22(11):1401–11.

    Article  PubMed  CAS  Google Scholar 

  44. Xu RQ, Blanvillain S, Feng JX, Jiang BL, Li XZ, Wei HY, et al. AvrACXcc8004, a type III effector with a leucine-rich repeat domain from Xanthomonas campestris pathovar campestris confers avirulence in vascular tissues of Arabidopsis thaliana ecotype Col-0. J Bacteriol. 2008;190(1):343–55.

    Article  PubMed  CAS  Google Scholar 

  45. Williams P. Quorum sensing, communication and cross-kingdom signalling in the bacterial world. Microbiology. 2007;153(Pt 12):3923–38.

    Article  PubMed  CAS  Google Scholar 

  46. Ryan RP, Fouhy Y, Lucey JF, Dow JM. Cyclic di-GMP signaling in bacteria: recent advances and new puzzles. J Bacteriol. 2006;188(24):8327–34.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  47. Ryan RP, McCarthy Y, Andrade M, Farah CS, Armitage JP, Dow JM. Cell-cell signal-dependent dynamic interactions between HD-GYP and GGDEF domain proteins mediate virulence in Xanthomonas campestris. Proc Natl Acad Sci U S A. 2010;107(13):5989–94.

    Article  PubMed  PubMed Central  Google Scholar 

  48. Tao F, He YW, Wu DH, Swarup S, Zhang LH. The cyclic nucleotide monophosphate domain of Xanthomonas campestris global regulator Clp defines a new class of cyclic di-GMP effectors. J Bacteriol. 2010;192(4):1020–9.

    Article  PubMed  CAS  Google Scholar 

  49. An SQ, Febrer M, McCarthy Y, Tang DJ, Clissold L, Kaithakottil G, et al. High-resolution transcriptional analysis of the regulatory influence of cell-to-cell signalling reveals novel genes that contribute to Xanthomonas phytopathogenesis. Mol Microbiol. 2013;88(6):1058–69.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  50. Guo Y, Zhang Y, Li JL, Wang N. Diffusible signal factor-mediated quorum sensing plays a central role in coordinating gene expression of Xanthomonas citri subsp. citri. Mol Plant Microbe Interact. 2012;25(2):165–79.

    Article  PubMed  CAS  Google Scholar 

Download references

Funding

This work was supported by the Guangxi Natural Science Foundation of China (2014GXNSFFA118005) and the Ba Gui Scholar Program of Guangxi Zhuang Autonomous Region of China (2014A002).

Availability of data and materials

All data generated or analyzed during this study are included in this published article and its Additional files 1, 2, and 3.

Consent for publication

Not applicable.

Author information

Authors and Affiliations

  1. State Key Laboratory for Conservation and Utilization of Subtropical Agro-bioresources, College of Life Science and Technology, Guangxi University, 100 Daxue Road, Nanning, 530004, Guangxi, China

    Bo-Le Jiang, Guo-Feng Jiang, Wei Liu, Li-Chao Yang, Li-Yan Yang, Lin Wang, Xiao-Hong Hang & Ji-Liang Tang

Authors
  1. Bo-Le Jiang
    View author publications

    You can also search for this author in PubMed Google Scholar

  2. Guo-Feng Jiang
    View author publications

    You can also search for this author in PubMed Google Scholar

  3. Wei Liu
    View author publications

    You can also search for this author in PubMed Google Scholar

  4. Li-Chao Yang
    View author publications

    You can also search for this author in PubMed Google Scholar

  5. Li-Yan Yang
    View author publications

    You can also search for this author in PubMed Google Scholar

  6. Lin Wang
    View author publications

    You can also search for this author in PubMed Google Scholar

  7. Xiao-Hong Hang
    View author publications

    You can also search for this author in PubMed Google Scholar

  8. Ji-Liang Tang
    View author publications

    You can also search for this author in PubMed Google Scholar

Contributions

JLT and BLJ designed all of the study. BLJ carried out the experiments, data analysis and the drafted manuscript. WL helped in RNA-deep sequencing. GFJ, LCY, and LYY helped in GUS assay and RT-PCR. LW helped in mutant library construction. XHH helped in plant assay. JLT and BLJ are the major contributors in writing the manuscript. All authors read and approved the final manuscript.

Corresponding author

Correspondence to Ji-Liang Tang.

Ethics declarations

Ethics approval and consent to participate

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Additional files

Additional file 1:

Table S1. RNA sequencing detail raw data. (XLS 8055 kb)

Additional file 2:

Table S2. Functional groups of RpfC- regulated genes. (DOCX 19 kb)

Additional file 3:

Table S3. Functional groups of RpfG- regulated genes. (DOCX 20 kb)

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Jiang, BL., Jiang, GF., Liu, W. et al. RpfC regulates the expression of the key regulator hrpX of the hrp/T3SS system in Xanthomonas campestris pv. campestris. BMC Microbiol 18, 103 (2018). https://doi.org/10.1186/s12866-018-1233-5

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: https://doi.org/10.1186/s12866-018-1233-5

Keywords

  • Xanthomonas
  • RpfC
  • hrpX

BMC Microbiology

ISSN: 1471-2180

Contact us