Many plant bacterial pathogens including Pseudomonas species, utilize the type III secretion system (T3SS) to deliver effector proteins into plant cells. Genes encoding the T3SS and its effectors are repressed in nutrient-rich media but are rapidly induced after the bacteria enter a plant or are transferred into nutrient-deficient media. To understand how the T3SS genes are regulated, we screened for P. savastanoi pv. phaseolicola (Psph) mutants displaying diminished induction of avrPto-luc, a reporter for the T3SS genes, in Arabidopsis. A mutant carrying transposon insertion into a gene coding for a small functional unknown protein, designated as rhpC, was identified that poorly induced avrPto-luc in plants and in minimal medium (MM). Interestingly, rhpC is located immediately downstream of a putative metalloprotease gene named rhpP, and the two genes are organized in an operon rhpPC; but rhpP and rhpC displayed different RNA expression patterns in nutrient-rich King’s B medium (KB) and MM. Deletion of the whole rhpPC locus did not significantly affect the avrPto-luc induction, implying coordinated actions of rhpP and rhpC in regulating the T3SS genes. Further analysis showed that RhpC was a cytoplasmic protein that interacted with RhpP and targeted RhpP to the periplasm. In the absence of RhpC, RhpP was localized in the cytoplasm and caused a reduction of HrpL, a key regulator of the T3SS genes, and also reduced the fitness of Psph. Expression of RhpP alone in E. coli inhibited the bacterial growth. The detrimental effect of RhpP on the fitness of Psph and E. coli required metalloprotease active sites, and was repressed when RhpC was co-expressed with RhpP. The coordination between rhpP and rhpC in tuning the T3SS gene expression and cell fitness reveals a novel regulatory mechanism for bacterial pathogenesis. The function of RhpP in the periplasm remains to be studied.
Many Gram-negative bacterial pathogens rely on the T3SS for successful infection of their hosts [1]. The T3SS is encoded by a cluster of hrp/hrc genes that are essential for the induction of a hypersensitive response (HR) in resistant and nonhost plants and pathogenicity in susceptible plants [2]. The T3SS functions as a conduit to deliver an array of effector proteins into plant cells [3]. The effectors interfere with the host defense systems and contribute to bacterial pathogenicity [4]. Some effectors elicit HR and disease resistance in plants containing cognate disease resistance genes, and are therefore named avirulence proteins [5]. The expression of hrp/hrc genes and the effector genes (together called T3SS genes hereafter) is coordinately regulated by various environmental and host factors [6]. T3SS genes are expressed at a very low level when grown in nutrient-rich medium, but quickly induced to high levels after the bacteria are infiltrated into plants or cultured in nutrient-deficient medium that is believed to resemble the environment of the plant intercellular spaces where the bacteria proliferate during infection [7,8]. As depicted in S1 Fig, the T3SS genes in P. syringae and P. savastanoi are activated by the extracytoplasmic function (ECF) -family alternate σ factor HrpL that recognizes a hrp box motif conserved in the promoters of many T3SS genes [9–11]. In turn, transcription of hrpL is controlled by a σ54-dependent promoter in an alternate σ factor RpoN-dependent manner [12]. Activation of hrpL also requires HrpR and HrpS, two homologous enhancer-binding proteins [13]. The hrpR and hrpS genes are in the same operon proceeded by the hrpR promoter [14]. HrpR and HrpS form a heterodimer that binds the hrpL promoter and induces hrpL transcription via interaction with the RpoN RNA polymerase holoenzyme [15,16]. The hrpRS operon is moderately expressed in KB and further induced in MM and in the plant [14–16]. A number of genes, including hrpA, aefR, and at least two two-component systems, gacAS and rhpRS, have been reported to regulate the transcription of the hrpRS operon [17–21]. hrpA encodes the T3SS pilus structural protein. Mutation of hrpA severely reduces the transcription of hrpRS, hrpL and T3SS genes [17]. AefR is a regulator of quorum sensing and epiphytic traits, and an aefR mutation reduces the hrpR promoter activity [18]. The GacAS system regulates multiple biological processes in various bacterial species, including motility, virulence, quorum sensing, and production of toxins, antibiotics, exopolysaccharides, and biofilms [19,20]. A mutation in the response regulator gene gacA severely reduces the expression of hrpRS and the downstream cascade genes [20]. Thus far, the mechanisms by which HrpA, AefR, and GacAS regulate the hrpRS expression remain unknown. RhpRS was identified as a negative regulator of the T3SS genes [21]. The response regulator RhpR, upon phosphorylation, binds a putative inverted repeat motif in the hrpR promoter and represses hrpRS transcription [21,22]. Dephosphorylation of RhpR reduces the binding affinity of RhpR to the hrpR promoter, and consequently the hrpRS promoter is de-repressed [21–23]. RhpS is a sensor kinase with dual activities. Under T3SS inducing conditions, RhpS presumably acts as a phosphatase that renders RhpR in the dephosphorylation state, which derepresses the hrpRS operon [21–23]. Another level of control of T3SS gene expression involves the stability of the HrpR protein, which is regulated by ATP-dependent protease Lon [24,25]. In a lon mutant, HrpR is stabilized, which elevates the expression of downstream genes [24,25]. The activity of HrpS is repressed by HrpV, a T3SS negative regulator that physically interacts with the HrpS protein [26]. HrpV-mediated repression can be suppressed by HrpG, a chaperone-like protein that interacts with HrpV [27]. The interaction of HrpG with HrpV liberates HrpS from the HrpV-repression and consequently up-regulates the T3SS cascade [27]. To investigate how Pseudomonas bacteria activate the T3SS genes in plants, a P. savastanoi pv. phaseolicola (Psph) mutant was isolated with diminished induction of avrPto-luc in Arabidopsis. We named the mutant gene rhpC (regulator of hrp, chaperone). rhpC is located immediately downstream of a putative metalloprotease gene that we called rhpP (regulator of hrp, protease). Here, we report the molecular and functional interactions between RhpP and RhpC in regulating the T3SS genes and bacterial fitness.
avrPto is a Pseudomonas T3SS effector gene carrying a typical hrp-box promoter [10]. In a previous study, we fused the avrPto promoter with the firefly luciferase gene luc in a broad host plasmid and constructed a reporter system for the T3SS gene expression in plants and MM [28]. To identify bacterial genes regulating the T3SS gene expression in plants, we constructed a transposon insertion mutant library in a Psph NPS3121 strain carrying the avrPto-luc reporter gene and screened for mutants with diminished avrPto-luc induction in Arabidopsis att1 plants [18,21]. att1 was previously isolated by our group, and it supported several-fold higher induction of avrPto and hrpL promoters than did the wild type Arabidopsis [28]. att1 plants provide a quick and sensitive reporter system for the assay of Pseudomonas T3SS gene regulation in plants [18,21,28]. The Psph NPS3121 strain is a non-host bacterium to Arabidopsis Col-0, and it does not multiply in the wild-type (WT) Col-0 and att1 plants [28,29]. Using the avrPto-luc reporter and att1 plants, we previously isolated a number of T3SS regulatory genes in the Psph NPS3121 strain, including aefR, rhpRS, hrpL, hrpR, and hrpS [18,21]. One Psph mutant we identified carried a transposon insertion in PSPPH2198 [30], which we later called rhpC because of its putative role as a molecular chaperone (Fig 1A). The mutant showed reduced induction of avrPto-luc not only in the att1 plant but also in MM (Fig 1B). A deletion mutant of rhpC (ΔrhpC) was subsequently constructed, and like the transposon insertion mutant, ΔrhpC also showed a reduction of the avrPto-luc activities in att1 and MM (Fig 1C and 1D). When inoculated into the wild-type Arabidopsis Col-0 plants, the ΔrhpC mutant also showed lower induction of avrPto-luc than did the wild-type strain (Fig 1E). The bacterial numbers of the wild-type Psph and the ΔrhpC mutant were similar and did not change clearly after inoculation into the Col-0 and att1 plants (S2 Fig). Therefore, the reduced avrPto-luc activity in the ΔrhpC mutant reflected the poor induction of the reporter gene in the plants. When inoculated into host bean plants, the ΔrhpC mutant displayed reduced bacterial growth (Fig 1F) and disease symptoms (Fig 1G). The avrPto-luc induction in Arabidopsis plants and MM as well as the bacterial growth and disease symptoms in bean plants were complemented by a broad host plasmid with a constitutive promoter expressing the wild-type rhpC gene in the ΔrhpC mutant (Fig 1C–1G). rhpC encodes a protein of 99 amino acid residues [30]. BlastP analysis identified homologous proteins of unknown function in a wide range of bacterial species (S3 Fig). A cytoplasmic localization of the RhpC protein was predicted by both CELLO [31,32] and PredictProtein (https: //predictprotein. org/). This small protein has an acidic isoelectric point (pI = 4. 73) and predominantly β-sheet and α-helical secondary structures (S4 Fig). rhpC is 20 bp downstream of PSPPH2199 (Fig 1A). PSPPH2199 encodes a protein of 356 amino acid residues [30]. BlastP analysis indicated that PSPPH2199 belongs to the metalloprotease of the M4 family [33]. We therefore named PSPPH2199 as RhpP. RhpP homologues exist not only in Pseudomonas (S5 Fig) but also in a wide range of other bacteria (S6 Fig). Proteins of this family have three Zn2+-binding amino acid residues, including two histidine residues in the HEXXH motif and a unique glutamate residue toward the C-terminal from the motif [33]. Protein alignment indicated that these residues (His176, His180 and Glu200) were all conserved in RhpP (S7 and S8 Figs). Additional residues at the RhpP active site were 146,147,173,177,191,240,241, and 279 (S7 and S8 Figs). Interestingly, all bacterial strains, except one (Desulfomonile tiedjei DSM 6799), that carry the RhpC homologue also carry the RhpP homologue (S5, S6 and S8 Figs), and the two genes are arranged in the same manner as in the Psph strain, suggesting co-evolution of the rhpPC locus. However, many bacterial species, including the plant bacterial pathogens Xanthomonas and Pectobacterium, carry only the RhpP homologue without RhpC (S5 and S6 Figs). The close proximity of rhpC and rhpP genes in the bacterial genome led us to test whether the two genes are co-transcribed into a polycistronic RNA. Total RNA was extracted from the NPS3121 strains cultured in KB and MM and reverse-transcribed with a primer derived from the 3' end of rhpC (S9 Fig). RT-PCR analysis using one primer derived from the 5' end of rhpP and another primer derived from the 3' end of rhpC (S9 Fig) produced a DNA fragment of the expected size (Fig 2A), indicating that the two genes are transcribed into a polycistronic RNA. The same RNA samples were also reverse-transcribed using primers specific for rhpC and rhpP, respectively. RT-PCR with rhpC- and rhpP-specific primers also detected the respective transcripts (Fig 2A). The different intensities of the RT-PCR products from the KB and MM cultures suggested possible differential regulation of rhpC and rhpP in response to different nutrient conditions (Fig 2A). To test this possibility, real-time PCR was performed to analyze the levels of rhpP and rhpC transcripts after reverse-transcription of the RNA samples with random primers, using 16S rRNA and rpoD as internal references. The rhpP RNA was more abundant in KB than in MM (Fig 2B and 2E), and rhpC showed the opposite expression patterns compared to rhpP (Fig 2C and 2F). The ratio of the rhpC/rhpP transcripts in KB was much lower than the ratio in MM (Fig 2D and 2G), suggesting that rhpP and rhpC were expressed not only as polycistronic RNA, but also in separate forms. The transcriptions of rhpP and rhpC were likely controlled by different promoters that were differentially regulated by nutrient conditions. Polycistronic genes are often functionally related. To test whether rhpP and rhpC are related in function, deletion mutants of the whole rhpPC locus and rhpP were created by homologous recombination. The resulting mutants were tested for avrPto-luc induction and bacterial virulence. Compared to the ΔrhpC mutant, the ΔrhpPC strain displayed better induction of avrPto-luc in both the att1 plants (Fig 3A) and MM (Fig 3B). In the host bean plants, the ΔrhpPC mutant displayed better bacterial growth and stronger disease symptoms than did the ΔrhpC mutant (Fig 3C and 3D). However, bacterial growth and disease symptoms in the host plants were repressed when a plasmid-borne rhpP under a constitutive promoter was expressed in the ΔrhpPC mutant (Fig 3C and 3D). Deletion of rhpP alone did not significantly affect the bacterial virulence, as shown by the similar disease symptoms induced by the wild-type strain and the ΔrhpP mutant in the host bean plants (Fig 3D). These results suggested that RhpP, when present alone in Psph, compromised the induction of the T3SS genes and bacterial virulence, and the presence of RhpC repressed the negative effect of RhpP. The sequence of rhpC predicts a cytoplasmic protein. To test this, we tagged RhpC at the C-terminus with HA and expressed the gene in the ΔrhpC mutant strain using a broad host plasmid. Bacterial protein was separated into periplasmic, membrane, and cytoplasmic fractions. Western blot analysis indicated that RhpC, like the cytoplasmic control protein RopA [34], was exclusively localized in the cytoplasm (Fig 4A). Metalloproteases of the M4 family in bacterial pathogens are largely secreted to the extracellular milieu by their host bacteria [35]. We therefore examined whether RhpP was also a secreted protein. RhpP was FLAG-tagged at the C-terminus in the broad host vector pHM1 under a constitutive promoter and expressed in the wide-type Psph strain. The resulting bacterium was cultured in KB and MM. The bacterial cells and culture media were then separated by centrifugation, the protein in the culturing media was precipitated by TCA, and the presence of RhpP-FLAG was examined using the anti-FLAG antibody. PSPPH_1783, which is homologous to the P. aeruginosa out-secreted protein PlcN/PlcH through the type II secretion pathway, was used as the secretion control in KB [36]. The T3SS effector AvrPto was used as a secretion control in MM [37]. Unlike the control proteins that were detected in the culture media, no RhpP-FLAG protein was detected in KB or MM, even when 500 mL of culture medium was used for protein precipitation (Fig 4B), indicating that RhpP was not secreted to the outside of the bacterial cells at the tested conditions. Sequence analysis of RhpP did not predict a membrane localization signal. The other possible compartment for RhpP localization would be the cytoplasm or periplasm. We therefore separated the bacterial cells into periplasmic and cytoplasmic fractions using osmotic shock. AmiC, a protein that is dispersed throughout the new-born cells and is secreted to the periplasm in divisional cells [38], was used to indicate the protein fractionation in periplasm. The cytoplasmic protein RpoA [34] was used as control of protein fractionation in cytoplasm. Western blot analysis indicated that the RhpP protein was present in both the cytoplasm and the periplasm in the WT strain (Fig 4C). As RhpC inhibited the function of RhpP, we asked whether RhpC affects the localization of RhpP. We therefore introduced the pHM1: : rhpP-FLAG plasmid into ΔrhpP, ΔrhpC, and ΔrhpPC mutants and examined the RhpP localization. RhpP was present in both the periplasm and the cytoplasm of the ΔrhpP mutant, but was detected only in the cytoplasm of the ΔrhpC and ΔrhpPC mutants (Fig 4C), suggesting that RhpC is required for the translocation of RhpP to the periplasm. We further tested whether RhpP translocation to the periplasm was through the general secretion pathway. As shown in Fig 4D, mutations of gspD and gspE genes of the general secretion pathway did not affect the RhpP localization in the Psph strain. The rhpP-FLAG gene expressed by the pHM1 plasmid under a constitutive promoter produced stronger protein signal in the WT Psph strain than in the ΔrhpC mutant (Fig 5A), suggesting that RhpC stabilized RhpP in the bacterium. This result and the functional interactions between RhpC and RhpP in regulating the T3SS genes and bacterial virulence raised the question whether RhpC physically interacts with RhpP. We tested this using the protein pull-down assay. RhpP-FLAG was expressed in the WT Psph strain using a plasmid and purified using anti-FLAG affinity gel. The E. coli BL21 strain expressing RhpC-GST or GST was sonicated, and the protein was purified with glutathione sepharose. RhpC-GST or GST on glutathione sepharose was further incubated with the RhpP-FLAG protein eluted from the anti-FLAG affinity gel. Western blot analysis showed that RhpP-FLAG was specifically pulled down by RhpC-GST (Fig 5B), indicating the physical interaction between RhpP and RhpC. Because RhpP is a putative metalloprotease, we hypothesized that, in the absence of RhpC, RhpP represses the T3SS gene expression by destabilizing the TTSS regulatory proteins. To test this, we compared the levels of three major T3SS regulatory proteins, HrpL, HrpR, and HrpS, in the WT, ΔrhpC, ΔrhpP, and ΔrhpPC strains. All these proteins were expressed under a constitutive promoter in the pHM1 plasmid. Western blot analysis revealed a lower level of HrpL protein in the ΔrhpC mutant than in other strains (Fig 6A), which was consistent with the lower T3SS gene expression in this strain. The levels of HrpR protein were similar in all the strains (Fig 6B), and so were the levels of HrpS protein (Fig 6C). The reduced level of HrpL protein in the ΔrhpC mutant might have resulted from degradation of HrpL by RhpP. To test this possibility, we purified HrpL-FLAG and RhpP-FLAG using anti-FLAG affinity gel. The purified proteins were incubated together in PBS buffer, and the levels of HrpL-FLAG protein were examined after 3 h of incubation. In the presence of PBS buffer only, HrpL-FLAG was stable (Fig 6D). However, the level of HrpL-FLAG was significantly reduced after incubation with RhpP-FLAG (Fig 6D). The reduction of HrpL-FLAG was much suppressed when EDTA, a metalloprotease inhibitor, was added with RhpP-FLAG, or when HrpL-FLAG was incubated with RhpPH279T, a RhpP mutant of the protease active site (Fig 6D). These results indicated that RhpP was an active metalloprotease for HrpL. To test whether RhpC had any effect on the RhpP protease activity, RhpC was added to the reaction. Co-incubation of RhpC with RhpP stabilized the HrpL-FLAG protein (Fig 6E), indicating that RhpC blocked the RhpP protease activity. We consistently observed smaller colonies of the ΔrhpC mutant than the WT, ΔrhpP, and ΔrhpPC strains on the KB plate. In liquid KB or MM culture, the ΔrhpC mutant also displayed slower growth, compared to the other three strains (Fig 7A and 7B). When RhpP was tagged with MBP in the pMAL-p2X plasmid and transformed into the E. coli BL21 strain, the resulting colonies were very small on the LB plate. Liquid LB medium inoculated with these small colonies stayed clear, even after 24 h of culture (Fig 7C). These results indicated that RhpP, when presented alone, was detrimental not only to the native bacterium but also to other bacterial species. To determine whether the detrimental effect of RhpP was related to the protease activity, amino acid residue His279 at the putative active site, was mutagenized to Asp and Thr. E. coli BL21 strains expressing the mutant recombinant proteins (RhpPH279D-MBP and RhpPH279T-MBP) showed normal growth in liquid LB culture (Fig 7C). The RhpPH279D and RhpPH279T proteins were also compared to RhpP when expressed in the ΔrhpPC strain. Unlike RhpP, neither RhpPH279D nor RhpPH279T affected the bacterial growth (Fig 7D; S10 Fig). Western blot analysis indicated that the RhpPH279D and RhpPH279T proteins were as stable as RhpP in the ΔrhpPC strain (Fig 7E). These results suggested that the negative effect of RhpP on bacterial growth was mediated by the protease activity. As RhpC inhibited the RhpP protease activity, and the Psph strain harboring the rhpPC locus was normal, we speculated that the presence of RhpC could repress the detrimental effect of RhpP on bacterial growth. This possibility was further tested by the co-expression of RhpC and RhpP in the E. coli BL21 strain. pMAL-p2X plasmid expressing RhpP-MBP, when introduced alone into BL21, severely inhibited the bacterial growth. However, when this plasmid was introduced into the BL21 strain expressing RhpC, the resulted bacterium grew normally both on the LB plate and in the LB liquid medium (Fig 7F). These results suggested that RhpC suppressed the detrimental effect of RhpP on bacterial fitness, probably by inhibiting the protease activity of RhpP in the cytoplasm. Given that RhpC interacts with RhpP and inhibits its protease activity, we wondered whether mutation of the active sites of RhpP interferes with the RhpC interaction. This was tested by protein pull-down assay between GST-RhpC and RhpP mutant proteins. In addition to RhpPH279D and RhpPH279T, we created another mutant with the three conserved zinc-binding residues all changed to Ala. As shown in Fig 8A, all the mutant proteins were pulled down specifically by GST-RhpC, indicating that the mutations of the active sites did not interrupt the interaction with RhpC. We also tested whether the mutations affected the RhpP protein translocation to the periplasm. As shown in Fig 8B, the mutant proteins, like the wild type RhpP, were also translocated to the periplasm.
In the search for genes regulating the T3SS genes in Psph, we identified the mutant of the rhpC gene with diminished T3SS gene induction and reduced pathogenicity in the host plant. rhpC is downstream of rhpP which encodes a putative metalloprotease. RhpC is a cytoplasmic protein that interacts with RhpP and facilitates the translocation of RhpP to the periplasm. The expression of RhpP alone in Psph and E. coli inhibited bacterial growth, and the inhibition was abolished by mutation of the conserved protease activity sites, suggesting that RhpP alone is an active protease in the bacterial cytoplasm. Purified recombinant RhpP protein can degrade HrpL in vitro, further showing RhpP as an active protease. The ΔrhpC mutant exhibited a reduced level of HrpL protein, the direct regulator of the T3SS genes. The reduction in HrpL was consistent with the reduced T3SS gene induction in the ΔrhpC mutant. Interestingly, the ΔrhpC mutant did not show a reduction in the HrpS and HrpR protein levels, suggesting that RhpP has substrate specificity. Nonetheless, HrpL is unlikely to be the only substrate for RhpP in the Psph cytoplasm, because hrpL- mutant did not show any growth defect in KB and MM [13,39]. In addition, RhpP probably degraded the E. coli proteins as well because expression of the RhpP-MBP recombinant protein in E. coli caused a severe growth defect, and the detrimental effect in E. coli required the protease active sites of RhpP. The reduced growth of the ΔrhpC mutant in the host plants was likely the result of reduced T3SS gene expression plus the reduced fitness of the bacterial cells. Protein localization analysis revealed that, in the WT Psph strain, an RhpP protein of the same size was present in the cytoplasm and the periplasm but not in the culture medium. This is different from the known RhpP homologues such as thermolysin from Bacillus thermoproteolyticus [40], elastase from Pseudomonas aeruginosa [41], Prt1 in Pectobacterium cratovorum [42], and many other M4 metalloproteases from other bacteria, which are all secreted proteins to extracellular milieu [35,43–45]. These extracellular proteases are encoded as inactive preproproteases with an N-terminal signal peptide that is followed by a propeptide and a catalytic domain. The signal peptides mediate the translocation of these preproproteases through the Sec pathway to periplasm, where the signal peptides are removed by the periplasmic-localized signal peptidase [35,43]. Immediately following the signal peptides are propeptides which are also called intramolecular chaperones [35,43]. Propeptides assist in the folding of the catalytic domains into active conformation [44,45]. Upon the completion of protein folding, propeptides are cleaved either by autoprocessing or with the help of other proteases [44]. The cleaved propeptide stays in contact with the catalytic domain, which stabilizes the substrate protein, prevents premature activation of the protease, and facilitates translocation of the protease through the outer membrane [46,47]. Alignment of RhpP with the out-secreted M4 metalloproteases showed a conserved C-terminal catalytic domain preceded by an N-terminal peptide of 67 amino acid residues. SignalP analysis did not find a signal peptide for the Sec pathway in the N-terminal sequence (S11 Fig). The propeptide sequences presented in the known M4 metalloproteases were not found in RhpP (S7 Fig). Consistently, mutations of the general secretion pathway genes gspD and gspE did not block the translocation of RhpP to the periplasm. Characterization of rhpC led us to propose that RhpC is a specific chaperone for RhpP. First, in almost all sequenced bacterial genomes carrying an RhpC homologue, the rhpC homologous gene is always coupled by the rhpP homologous gene, suggesting co-evolution of the two genes. Second, RhpC is a small cytoplasmic protein (molecular mass = 11 kDa) with a relatively low isoelectric point and a C-terminal helical structure. These characteristics are also shared by many other chaperones [48,49]. In addition, RhpC is required for RhpP protein stability and translocation from the cytoplasm to the periplasm. The presence of RhpC inhibited the RhpP protease activity and the detrimental effect of RhpP on bacterial fitness, suggesting that RhpC is required for the proper function of RhpP. The interaction of RhpC with RhpP in the protein pull-down assay provided further evidence that RhpC is the chaperone of RhpP. Based on these characteristics, RhpC appears to be a functional mimic of prepropeptides of the out-secreted metalloproteases. Although RhpC can inhibit the protease activity of RhpP, mutations of the protease active sites (His176, Glu177, His180, and His279) in RhpP did not abolish the interaction with RhpC, suggesting that these active sites are probably not at the RhpC-interacting surface. These RhpP mutant proteins were also translocated to the periplasm in the presence of RhpC. It is possible that the RhpC interaction changes RhpP to an inactive conformation that is compatible with the translocation through the bacterial inner membrane. Gram-negative bacteria have five classes of protein secretion systems spanning both the inner membrane and the outer membrane that deliver cytoplasmic proteins to the outside of the bacterial cell, including type I secretion system (T1SS), T2SS, T3SS, T4SS, and T6SS [50]. However, only two classes of protein transporters have been reported that span the inner membrane and deliver proteins to the periplasm, including the Sec apparatus and the Tat system (twin-arginine translocation system) [50,51]. The involvement of the Sec pathway in RhpP translocation was ruled out because deletion of gspE (secE) did not block the RhpP translocation to the periplasm. Proteins targeting to the Tat machinery usually have signal peptides that contain a conserved twin-arginine motif [51]. TatP analysis predicted a low Tat-targeting signal and a peptide cleavage site between A49 and R50 in the N-terminus of RhpP (S12 Fig). However, the same molecular weight of RhpP detected by Western blot in cytoplasm and periplasm did not support the cleavage of the signal peptide. Because RhpC interacts with RhpP and is required for RhpP translocation, we wondered if RhpC has a signal peptide for the Tat system and carries RhpP to the Tat system in a" piggy-back" manner. However, we did not find the twin-arginine signal peptide in RhpC. Instead, we found significant similarity between RhpC and TatB of the Tat system (S13 Fig). The functional significance of this sequence similarity is unknown. Whether RhpP passes through the cytoplasmic membrane through the Tat system remains to be investigated. Real-time PCR analysis indicated that the rhpPC locus is subjected to complex regulation in response to nutrient conditions. This locus is transcribed not only into rhpPC polycistronic RNA but also into discrete rhpC RNA. The rhpP (or rhpPC) RNA is more abundant in KB than in MM, opposite to rhpC that is expressed at a higher level in MM than in KB. The ratio of rhpC/rhpP transcripts is also much higher in MM than in KB. Given the facts that RhpP in cytoplasm can degrade the HrpL protein and that the RhpP protease activity can be repressed by RhpC, we propose that the reduced rhpP transcripts and induced rhpC transcripts in MM serve as double protection that restricts the detrimental RhpP activity to a minimal level in the cytoplasm, which in turn secures the high induction of the T3SS genes. It is worthwhile to mention that the negative regulation of RhpP on the T3SS gene induction is obvious only when RhpC is absent, because deletion of the rhpPC locus did not significantly change the induction of avrPto-luc in the plant and MM. Thus, it is the coordination between rhpP and rhpC that plays a critical role in regulating the T3SS gene induction. It appears that RhpC, as a chaperone, keeps the function of RhpP under control in the cytoplasm by inhibiting the RhpP protease and facilitating its translocation to the periplasm. RhpP may play an important role in periplasmic protein quality control by degrading the functionally abnormal proteins of bacterium or imported peptides from environment. We conducted a preliminary analysis to compare the proteomes of the wild-type Psph and ΔrhpC strains, which revealed ~30 periplasmic proteins that were >1. 5 fold more abundant in the ΔrhpC mutant (S1 Table). Most of these periplasmic proteins are ABC transporters involved in transportation of various small molecules. Whether any of these differentially expressed proteins are direct substrates of RhpP remains to be studied. Nonetheless, the presence of RhpP protein in the periplasm and cytoplasm in the wild-type Psph strain implies that the regulation of T3SS genes is coordinated with the periplasmic activities. RhpC plays a key role in protecting the T3SS regulation pathway and bacterial fitness from the detrimental effect of RhpP by directly inhibiting the RhpP protease activity in bacterial cytoplasm and targeting RhpP to the periplasm. The coordination of the two-component rhpPC module represents a novel mechanism underlying the fine regulation of T3SS genes in response to growth conditions.
Arabidopsis att1 mutant plants [28] were used for the screening of Psph mutants with diminished induction of the avrPto-luc reporter. Bean (Phaseolus valgaris cv. Red Kidney) [52] was used for pathogenicity assays. Growth of plant materials was as described previously [21]. All Psph mutants were derived from the NPS3121 strain. E. coli DH5α was used for constructing all plasmids. E. coli BL21 was used for expression of recombinant proteins. NPS3121 and its derivatives were grown at 28°C in KB medium [53] containing appropriate antibiotics. E. coli strains were cultured in Luria-Bertani (LB) medium at 37°C. Antibiotics for selection of Psph strains were rifampicin, 25 mg/liter; kanamycin, 10 mg/liter; gentamicin, 10 mg/liter; and spectinomycin, 50 mg/liter. Antibiotics for selection of E. coli were ampicillin, 100 mg/liter; kanamycin, 50 mg/liter; spectinomycin, 100 mg/liter; and gentamicin, 20 mg/liter. Psph NPS3121 strain carrying the pHM2: : avrPto-luc reporter plasmid was used for construction of the EZ Tn5<KAN-2> (Epicentre, Madison, WI, U. S. A.) transposon insertion library, as described by Xiao et al. [21]. Briefly, electro-competent cells were mixed with transposon and transposase as instructed by the manufacturer. Following electroperation, the NPS3121 mutant library was plated on KB medium containing 10 mg of kanamycin per liter (selection for EZ: : TN<KAN-2> transposon) and 10 mg of spectinomycin per liter (selection for pHM2: : avrPto-luc plasmid). To screen the mutants regulating avrPto-luc reporter in plant, the NPS3121 mutant colonies were grown overnight at 25°C in liquid KB medium containing spectinomycin and kanamycin. The bacteria were washed twice with sterile water, and then suspended in sterile water to optimal density at 600 nm (OD600) = 0. 5 for inoculation. Six hour after injection into Arabidopsis att1 plants, the inoculated leaves were excised and sprayed with 1 mM luciferin dissolved in 0. 01% Tween-20, and the luciferase activity was determined using a cooled charge-couple device (CCD, Roper Scientific, Trenton, NJ, U. S. A.). A total of 6,000 colonies were screened. The transposon insertion sites were determined by a two stage semi-degenerated PCR, as described by Xiao et al [21]. To confirm the transposon insertion site in rhpC- mutant, gene-specific primer rhpC-R and transposon-specific primer Kan2-SP3 were used to PCR amplify the transposon-flanking DNA. The PCR product was sequenced to determine the transposon insertion site. Bacteria containing the avrPto-luc reporter gene were grown in KB with appropriate antibiotics to OD600 = 2. The bacteria were washed twice with sterile water, and then resuspended in sterile water to OD600 = 0. 5. To measure the reporter gene activity in plant, bacteria at OD600 = 0. 5 were injected into Arabidopsis att1 plants. The inoculated leaves were excised 6 h after injection and sprayed with 1 mM luciferin dissolved in 0. 01% Tween-20, and the luciferase activity was determined using a cooled CCD (Roper Scientific, Trenton, NJ, U. S. A.). To measure the reporter gene activity in MM, bacteria were grown in KB with appropriate antibiotics overnight to OD600 = 2. 0, washed three times with sterile water, resuspended in MM with appropriate antibiotics to OD600 = 0. 1, and then cultured at 28°C with constant shaking for 6 h before the measurement. Bacterial culture (100 μl) was mixed with 1 μl of 1 mM luciferin in a 96-well plate, and the luciferase activities were determined using a cooled CCD (Roper Scientific, Trenton, NJ, U. S. A.). The luciferase activities of all measurements were normalized to the bacterial numbers. An F test (P < 0. 05) was conducted to all quantitative experiments. Preparation of bacterial inoculum and bacterial growth assay were as previously described [21]. Psph NPS3121 wild type and mutant strains at 2×105 CFU/ml were hand-injected into the primary leaves of 10-day-old bean plants. Bacterial growth were measured at 0,2, and 4 days after inoculation. Disease symptoms on bean leaves were photographed 7 days after inoculation. Oligo primers and plasmids used in this study are listed in S2 and S3 Tables, respectively. pBluescript-HA was modified from pBluescript-SK (+) in our previous study [21] and used for HA-tagging of genes at the 3′ end. Broad host plasmids pML122 [54] and pHM1 [55] with strong constitutive promoters were used to express genes in NPS3121 strain. To construct the pML122: : rhpC-HA plasmid, the rhpC gene from the NPS3121 strain was PCR-amplified using the RhpC-HA primer pair. The PCR product was digested with HindIII and NheI and cloned into the pBluescript-HA plasmid predigested with the same enzymes. After sequence confirmation, the pBluescript: : rhpC-HA plasmid was digested by HindIII and BamHI, and the insert was subsequently cloned into pML122 predigested with the same enzymes, resulting in pML122: : rhpC-HA. To construct the pHM1: : rhpP-FLAG plasmid, the rhpP gene of the NPS3121 strain was PCR-amplified using the RhpP-FLAG (containing FLAG-tag DNA sequence) primer pair. The PCR product was digested with EcoRI and HindIII and cloned into the pGEM-T plasmid predigested with the same enzymes. After sequence confirmation, the pGEM-T: : rhpP-FLAG plasmid was digested by EcoRI and HindIII, and the insert was subsequently cloned into pHM1 predigested with the same enzymes, resulting in pHM1: : rhpP-FLAG. To construct the pHM1: : hrpL-FLAG plasmid, the hrpL gene from the NPS3121 strain was PCR-amplified using the HrpL-FLAG (containing FLAG tag DNA sequence) primers. The PCR product was digested with HindIII and EcoRI and cloned into the pGEM-T plasmid predigested with the same enzymes. After sequence confirmation, the pGEM-T: : hrpL-FLAG plasmid was digested by HindIII and EcoRI, and the insert was subsequently cloned into pHM1 predigested with the same enzymes, resulting in pHM1: : hrpL-FLAG. To construct the pHM1: : hrpS-FLAG plasmid, the hrpS gene from the NPS3121 strain was PCR-amplified using the HrpS-FLAG (containing FLAG tag DNA sequence) primers. The PCR product was digested with EcoRI and HindIII and cloned into the pGEM-T plasmid predigested with the same enzymes. After sequence confirmation, the pGEM-T: : HrpS-FLAG plasmid was digested by EcoRI and HindIII, and the insert was subsequently cloned into pHM1 predigested with the same enzymes, resulting in pHM1: : hrpS-FLAG. To construct the pHM1: : hrpR-HA plasmid, the hrpR gene from the NPS3121 strain was PCR-amplified using the HrpR-HA (containing HA-tag DNA sequence) primers. The PCR product was digested with PstI and HindIII and cloned into the pGEM-T plasmid predigested with the same enzymes. After sequence confirmation, the pGEM-T: : hrpR-HA plasmid was digested by PstI and HindIII, and the insert was subsequently cloned into pHM1 predigested with the same enzymes, resulting in pHM1: : hrpR-HA. To construct the pHM1: : PSPPH_1783-FLAG, pHM1: : AmiC-FLAG, pHM1: : RpoA-FLAG plasmid, the PSPPH_1783, AmiC (PSPPH_5159), RpoA (PSPPH_4567) were amplified from the NPS3121 strain by PCR and cloned into pHM1 using a ClonExpress II One Step Cloning Kit (Vazyme Biotech, Nanjing, China). To construct the pGEX3X: : rhpC-GST plasmid, the rhpC gene from the NPS3121 strain was PCR-amplified using the RhpC-GST primers. The PCR product was digested with BamHI and EcoRI and cloned into the pGEM-T plasmid predigested with the same enzymes. After sequence confirmation, the pGEM-T: : rhpC plasmid was digested by BamHI and EcoRI, and the insert was subsequently cloned into pGEX3X predigested with the same enzymes, resulting in pGEX3X: : rhpC-GST. To construct the pMAL-p2X: : rhpP-MBP plasmid, the rhpP gene from the NPS3121 strain was PCR-amplified using the RhpP-MBP primers. The PCR product was digested with EcoRI and BamHI and cloned into the pGEM-T plasmid predigested with the same enzymes. After sequence confirmation, the pGEM-T: : rhpP-MBP plasmid was digested by EcoRI and BamHI, and the insert was subsequently cloned into pMAL-p2X predigested with the same enzymes, resulting in pMAL-p2X: : rhpP-MBP. To construct the ΔrhpP mutant, a 1. 5-kb DNA fragment upstream of the rhpP open reading frame (ORF) was PCR-amplified using primers RhpP-FlankA (EcoRI and BamHI). A 1-kb DNA fragment downstream of rhpP ORF was PCR-amplified using primers RhpP-FlankB (BamHI and HindIII). The PCR products were digested with EcoRI and BamHI and BamHI and HindIII, respectively, and were ligated into pGEM-T, resulting in pGEM-T: : rhpPFlankA and pGEM-T: : rhpPFlankB. After sequence confirmation, the pGEM-T: : rhpPFlankA and pGEM-T: : rhpPFlankB plasmids were digested by EcoRI and BamHI and BamHI and HindIII, and the inserts were subsequently cloned into pK18mobsacB [56], resulting in pK18mobsacB: : rhpPFlankAB. This plasmid was then transformed into E. coli S17-1 which was used as a donor strain, and NPS3121 was used as a recipient strain. Both recipient strain and donor strain were cultured overnight, and then 50 μl of each were mixed and incubated for 2 days at 28°C. The bacteria were then collected and plated onto the KB plate containing rifampicin and kanamycin. After 2 days incubation, the rifampicin and kanamycin resistant colonies were single crossover merodiploid transconjugants. Pick several colonies and suspend the cells in a new tube and plate the suspension onto the KB/ rifampicin 10% sucrose plate. The sucrose rifampicin resistant colonies were regarded as the deletion mutant and further verified by PCR and sequencing. To construct the ΔrhpC mutant, a 1. 5-kb DNA fragment upstream of rhpC ORF was PCR-amplified using primers RhpC-FlankA (EcoRI and BamHI). A 1-kb DNA fragment downstream of rhpC ORF was PCR-amplified using primers RhpC-FlankB (BamHI and HindIII). The PCR products were digested with EcoRI and BamHI and BamHI and HindIII, respectively, and were ligated into pGEM-T, resulting in pGEM-T: : rhpCFlankA and pGEM-T: : rhpCFlankB. After sequence confirmation, the pGEM-T: : rhpCFlankA and pGEM-T: : rhpCFlankB plasmids were digested by EcoRI and BamHI and BamHI and HindIII, and the inserts were subsequently cloned into pK18mobsacB, resulting in pK18mobsacB: : rhpCFlankAB. The remaining procedures were the same as described for construction of the ΔrhpP mutant. To construct the ΔrhpPC mutant, a 1. 5-kb DNA fragment upstream of rhpP ORF was PCR-amplified using primers RhpP-FlankA (EcoRI and BamHI). A 1-kb DNA fragment downstream of rhpC ORF was PCR-amplified using primers RhpC-FlankB (BamHI and HindIII). The PCR products were cloned into pK18mobsacB, resulting in pK18mobsacB: : rhpCFlankAB. The remaining procedures were the same as described for construction of the ΔrhpP mutant. The same procedures described above were also used for construction of the ΔgspD and ΔgspE deletion mutants, except different primers were used to amplify DNA flanking the corresponding genes. Primers GspD-FlankA and GspD-FlankB were used for construction of ΔgspD, and primers GspE-FlankA and GspE-FlankB were used for construction of ΔgspE. To generate RhpPH279D, RhpPH279T, and RhpPH176A, E177A, H180A mutants, primer sets (RhpPH279D, RhpPH279T, and RhpPH176A, E177A, H180A) containing corresponding mutations and the pGEM-T: : rhpP-FLAG construct as template were used in PCR with the high fidelity DNA polymerase Phusion (Thermo Scientific, Waltham, MA, U. S. A.). The PCR product was digested with DMT enzyme (Transgen Biotech, Beijing, China) and then transformed into E. coli. Mutations in the resulting clones were verified by sequencing. Bacterial RNA was extracted using a modified hot phenol method [57]. RQ1 DNase (Promega, Madison, WI, U. S. A.) treatment was used to remove the contaminating DNA in RNA samples. Real-time PCR assay of gene expression was performed as described [58]. Briefly total RNA (10 μg) was reverse-transcribed using random primers. The reactions were first treated with RNase and then used as template for real-time PCR analyses with primer pairs rhpP-5' /-3 and rhpC-5' /-3 for rhpP and rhpC respectively, and primer pairs 16S rRNA, recA, and rpoD as internal controls. The relative expression levels of rhpP and rhpC were normalized to 16S rRNA, rpoD and recA. E. coli BL21 strains containing pGEX-3X-rhpC and pGEX-3X plasmids were cultured in LB at 37°C to OD600 = 0. 5 before adding 1 mM IPTG. The bacteria were then cultured overnight at 16°C to induce the production of the recombinant proteins. RhpC-GST and GST were purified using the Glutathione Sepharose ™ 4B (GE Healthcare Bio-Science AB, Uppsala, Sweden), following the manufacture’s instruction. The wild type Psph strains containing the pHM1: : rhpP-FLAG, pHM1: : rhpPH279D-FLAG, pHM1: : rhpPH279T-FLAG, and pHM1: : phpPH176A, E177A, H180A- FLAG were used to produce the corresponding RhpP and mutant proteins. The bacteria were cultured in 200 ml KB/rifampicin and spectinomycin at 28°C with constant shaking at 220 rpm. The bacteria were washed once with ice-cold PBS (10 mM Tris-HCl pH8. 0,1 mM EDTA pH 8. 0,150 mM NaCl), sonicated in ice-cold PBS, and then centrifuged at 4°C and 10,000 x g for 30 min. The supernatant was mixed with 1/1000 PBS-pre-washed anti-FLAG M2 Affinity Gel (Sigma Aldrich, St. Louis, MO, U. S. A.) and incubated at 4°C for 2 h with constant shaking. RhpP-FLAG protein bound to the beads was centrifuged, washed three times with PBS, and the protein was then washed off the beads using 3×FLAG peptide (200 μg/ml). The purified protein was examined using Western blot. RhpC-GST or GST bound to the Glutathione Sepharose beads was mixed with the purified RhpP-FLAG protein and incubated at 4°C for 2 h with constant shaking. Aliquot a small volume as input. The remaining of the mixture was centrifuged at 50 x g for 5 min, the precipitate was then washed three times (each time for 5 min) with ice-cold PBS, and then three times (each time for 5 min) with ice-cold wash solution (10 mM Tris-HCl pH8. 0,1 mM EDTA pH 8. 0, and 500 mM NaCl). Protein bound to the beads were eluted with elution buffer (20 mM reduced glutathione, 50 mM Tris-HCL pH 8. 0) and analyzed with Western blot as previously described [21]. The procedures described previously [59,60] were applied for periplasmic and cytoplasmic protein assay. Bacteria cultured in KB or MM were centrifuged and then suspended in ice-cold osmotic solution II (OS II: 20 mM Tris-HCl, pH8. 0; 2. 5 mM EDTA; 2 mM CaCl2) to OD600 = 3. 0. Aliquot 10 μl of the bacterial suspension and slowly add in 1 ml ice-cold osmotic solution I (OS I: 20 mM Tris-HCl, pH8. 0; 2. 5 mM EDTA; 2 mM CaCl2; 20% (w/v) sucrose). After 10 min of incubation in ice, the bacteria were centrifuged and then suspended in 1 ml ice-cold OS II, and continued incubation in ice for 20 min. Periplasmic contents defused into the solution during the incubation was collected by centrifugation. The bacterial pellet was suspended in 1 ml OS II. Cytoplasmic protein were released into solution by sonication and collected by ultracentrifugation. To test protein secretion into the culture medium, bacteria were first cultured in 10 ml KB medium to OD600 = 2, and then transferred into 500 ml KB for continuing culture to OD600 = 1. For secretion assay in KB medium, the bacteria were separated from the KB medium by centrifugation. For secretion assay in MM, the 500 ml KB culture were centrifuged, and the bacteria were washed three times with MM and then suspended in 500 ml MM. After 6 h culture in MM, the bacteria were separated from the MM by centrifugation. The medium was filtrated with the 0. 45 μM membrane to remove the bacterial residuals, and then mixed with equal volume of ice-cold 20% TCA. After 30 min incubation in ice, the mixture was centrifuged at 10,000 x g for 15 mins, and the pellet was washed three times with ice-cold acetone, and then boiled in SDS sample buffer for Western blot analysis. RhpP-FLAG and RhpPH279T-FLAG proteins were produced by pHM1: : rhpP-FLAG and pHM1: : rhpPH279T-FLAG plasmids, respectively, in Psph strain. HrpL-FLAG protein was produced by the pHM1: : hrpL-FLAG plasmid in E. coli BL21 strain. The proteins were purified by the anti-FLAG M2 Affinity Gel and eluted using 3×FLAG peptide (200 μg/ml). RhpC-GST and GST were purified using glutathione Sepharose beads. The purified HrpL-FLAG protein was adjusted to a concentration of 200μg/ml in PBS buffer, and all the other purified were adjusted to a concentration of 400μg/ml in PBS buffer. For each reaction, 50 μl of purified HrpL-FLAG protein was mixed with equal volume of PBS buffer or other purified proteins. EDTA was added to a final concentration of 5mM. Aliquot of 50 μl was taken from each reaction and mixed with SDS sample buffer as 0 h control, and the remaining volumes were incubated at 28°C for 3 h before examined by Western blot analysis. SDS-PAGE and Western blot analysis was conducted according to the procedures described previously [21]. Anti-FLAG antibody and anti-HA antibody were purchased from Sigma Aldrich (St Louis, MO, USA) and Abmart (Shanghai, China), respectively. Homologous sequences of RhpC and RhpP were downloaded from EnsemblBacteria [61] (http: //bacteria. ensembl. org/index. html) and the Pseudomonas Genome [62] (http: //pseudomonas. com/) databases with RhpC and RhpP from P. s. pv. phaseolicola 1448A as queries. All the sequences were aligned with ClustalW, and the UPGMA phylogenetic tree were then constructed with MEGA5 using default parameters [63]. The isoeletric point of RhpC protein was calculated with 15 methods included in Isoelectric Point Calculator (IPC, http: //isoelectric. org/calculate. php). The secondary structure of RhpC was predicted with PredictProtein (https: //predictprotein. org/), the most widely used server for structure prediction. SignalP [64] (http: //www. cbs. dtu. dk/services/SignalP/) and TatP [65] (http: //www. cbs. dtu. dk/services/TatP/) were used to predict the signal peptide and possible Tat-targeting peptide in RhpP proteins based on the classifications of bacteria. Two widely used online servers, CELLO [31,32] (http: //cello. life. nctu. edu. tw/) and PredictProtein (https: //predictprotein. org/), were used to predict the subcellular location of RhpC.
The induction of the type III secretion system (T3SS) is of great importance to the pathogenesis of bacterial pathogens in host plants. Pseudomonas savastanoi pv. phaseolicola (Psph) causes halo blight disease on beans. We discovered that the bicistronic genes in the rhpPC locus of Psph act coordinately to regulate the T3SS gene expression, bacterial fitness, and pathogenicity. rhpP encodes a metalloprotease that can degrade the key T3SS regulator protein HrpL and reduce bacterial fitness. rhpC encodes a chaperone that inhibits the RhpP activity and mediates translocation of RhpP to the periplasm. The level of rhpP RNA is high in KB but decreases in MM, but the rhpC RNA is low in KB but increases in MM. The elevated rhpC/rhpP transcript ratio in MM plus the inhibition of RhpC on RhpP activity in cytoplasm provide double insurance that warrants high induction of the T3SS genes in MM and bacterial fitness. The coordination between rhpP and rhpC reveals a new mechanism regulating bacterial pathogenicity, and may provide an important target for controlling bacterial pathogens.
Two components of the rhpPC operon coordinately regulate the type III secretion system and bacterial fitness in Pseudomonas savastanoi pv. phaseolicola