Journal of Bacteriology, June 2004, p . 3304-3312, Vol . 186, No . 11

Isolation and Characterization of rpoS from a Pathogenic Bacterium, Vibrio vulnificus: Role of ^S in Survival of Exponential-Phase Cells under Oxidative Stress

Kyung-Je Park,¹ Min-Jin Kang,^1, Songhee H . Kim,² Hyun-Jung Lee,¹ Jae-Kyu Lim,¹ Sang Ho Choi,³ Soon-Jung Park,⁴ and Kyu-Ho Lee^1*

Department of Environmental Science, Hankuk University of Foreign Studies, Yongin, Kyunggi-Do 449-791,¹ Department of Food Science and Technology, Seoul National University, Seoul 151-742,³ Department of Parasitology, Yonsei University College of Medicine, Seoul 133-791, South Korea,⁴ Department of Cell Biology and Molecular Genetics, University of Maryland at College Park, College Park, Maryland²

Received 3 September 2003/ Accepted 24 February 2004

 
A gene homologous to rpoS was cloned from a fatal human pathogen, Vibrio vulnificus . The functional role of rpoS in V . vulnificus was accessed by using an rpoS knockout mutant strain . This mutant was impaired in terms of the ability to survive under oxidative stress, nutrient starvation, UV irradiation, or acidic conditions . The increased susceptibility of the V . vulnificus mutant in the exponential phase to H₂O₂ was attributed to the reduced activity of hydroperoxidase I (HPI) . Although ^S synthesis was induced and HPI activity reached the maximal level in the stationary phase, the mutant in the stationary phase showed the same susceptibility to H₂O₂ as the wild-type strain in the stationary phase . In addition, HPII activity, which is known to be controlled by ^S in Escherichia coli, was not detectable in V . vulnificus strains under the conditions tested . The mutant in the exponential phase complemented with multiple copies of either the rpoS or katG gene of V . vulnificus recovered both resistance to H₂O₂ and HPI activity compared with the control strain . Expression of the katG gene encoding HPI in V . vulnificus was monitored by using a katG::luxAB transcriptional fusion . The expression of this gene was significantly reduced by deletion of ^S in both the early exponential and late stationary phases . Thus, ^S is necessary for increased synthesis and activity of HPI, and ^S is required for exponentially growing V . vulnificus to develop the ability to survive in the presence of H₂O₂ .

 
The life cycles of pathogenic bacteria involve periods in which they exist in a nongrowing state in stressed environments . Only if they survive such conditions are they able to proliferate with high metabolic activity in the proper host environments (7, 36) . Thus, these organism have evolved several mechanisms that allow them to survive under stressful conditions, such as starvation, temperature fluctuation, oxidative stress, and osmotic shock, and that enable them to resume growth once the stress is removed (27) . The cellular responses to environmental stimuli have been extensively studied in many bacterial species, most notably Escherichia coli .

To respond properly to diverse stresses, E . coli requires the rpoS gene product, which is a second principal sigma factor (^S); this product induces expression of many genes and allows the organism to mediate changes in cellular physiology and structure and to adapt, resist, and survive under stress conditions (9, 16, 19). ^S is also required for eliciting phenotypes related to virulence in many pathogenic bacteria belonging to the subdivision of Proteobacteria (21, 32, 39, 45, 50) .

It is generally believed that most microorganisms that communicate with, associate with, or colonize host animals are relatively well equipped with defense mechanisms to deal with oxidative stress (6, 15, 43) . E . coli produces at least two enzymes to overcome the presence of hydrogen peroxide and to maintain a relatively constant concentration of intracellular H₂O₂ (8); these enzymes are KatG (hydroperoxidase I [HPI]), which has both catalase and peroxidase activities, and monofunctional KatE (HPII), which has catalase activity (25) . KatG, one of the members of the OxyRS regulon, is induced by direct exposure to H₂O₂ (37) . In contrast, KatE is known to be regulated by ^S, and consequently cellular expression of this enzyme increases at the onset of the stationary phase (25, 30) . Open reading frames homologous to both katG and katE are present in the genomes of Vibrio cholerae and Vibrio parahaemolyticus . The presence and role of monofunctional catalases have been studied in Vibrio fischeri and Vibrio rumoiensis, but the regulation of these enzymes has not been described (11, 44, 51) .

The causative agent of septicemia, Vibrio vulnificus, has been considered an important pathogen in humans due to its rapid pathogenic progress and its high mortality rate (10, 38) . A number of studies have been performed on virulence factors of this organism, including metalloprotease (13), hemolysin (48), and siderophores (35) . Several regulators, including cyclic AMP receptor protein (CRP)/LuxR (12, 33), ToxRS/CRP (1, 17), and Fur (18), have been reported to control expression of these virulence factors . While survival of this bacterial species has been studied under diverse conditions (26), the molecular mechanisms underlying its survival strategies have not been studied well .

In an effort to isolate global regulators involved in survival of V . vulnificus, we cloned the rpoS gene and defined its physiological role in survival of V . vulnificus in the presence of various stresses . These analyses showed that V . vulnificus in the exponential phase requires ^S for survival in the presence of low concentrations of hydrogen peroxide . In the present study we also observed regulation of the expression and activity of a catalase involved in this response, and the results were quite different from those obtained with E . coli .

 
Isolation of the rpoS gene from V . vulnificus. The genomic DNA of V . vulnificus ATCC 29307 was prepared by a standard technique (29) and then partially digested with Sau3AI and size fractionated by agarose gel electrophoresis . The DNA fragments, which ranged from 2 to 6 kb long, were pooled and ligated with the pUC19 vector which had been digested with BamHI and subsequently treated with bacterial alkaline phosphatase . The V . vulnificus library obtained was introduced into E . coli ZK918 having a deletion in its rpoS gene and a ^S-dependent bolA::lacZ fusion in its chromosome (2) . After transformation with the library, colonies were screened on Luria-Bertani (LB) medium supplemented with ampicillin (100 µg/ml) and X-Gal (5-bromo-4-chloro-3-indolyl-ß-D-galactopyranoside) (10 µg/ml), which was blue as a result of induced expression of bolA::lacZ after addition of the RpoS homolog of V . vulnificus . Sequencing of the double-stranded DNA of the plasmid selected, pINE32, containing a 2,693-bp insert, was performed with an Applied Biosystems 373A automated DNA sequencer . The remaining gaps in the sequence were filled in by sequence analysis by using specifically designed internal primers that annealed to the insert region . Sequence analysis and database searches were performed by using the National Center for Biotechnology Information BLAST server .

Construction of rpoS knockout mutant KPR101. A 762-bp NruI fragment containing two-thirds of the rpoS coding sequence was deleted from pINE32 . The resultant plasmid, pKP11, was digested with SmaI and XbaI, which resulted in a DNA fragment containing a region adjacent to the rpoS gene but not the rpoS gene . This DNA was cloned into suicide vector pDM4 (23), which was digested with ApaI and XbaI, yielding pKP13 . pKP13 in E . coli SM10 pir was mobilized into strain AR, a rifampin-resistant derivative of the wild-type strain V . vulnificus ATCC 29307 . Conjugal transfer was performed by mixing aliquots of the strains that contained about 10⁸ donor cells and about 10⁸ recipient cells and then incubating the preparation overnight at 37°C in close contact on a membrane filter . The cell mixture was then resuspended in LBS (LB medium containing NaCl at a final concentration of 2.5%) broth and plated onto selective plates (LBS agar plates supplemented with 4 µg of chloramphenicol per ml and 50 µg of rifampin per ml) . A colony showing indications of a double homologous recombination event (resistance to 5% sucrose and sensitivity to chloramphenicol) was isolated, and deletion of its rpoS region was confirmed by PCR by using primers F2 and R2 (Table 1) .

 
Determination of survival of V . vulnificus under various stress conditions. Exponential-phase cultures (optical density at 600 nm [OD₆₀₀] in LBS broth, 0.15 to 0.3) or stationary-phase cultures (OD₆₀₀ in LBS broth, about 3 to 4; usually 8 to 10 h after an overnight culture was added to fresh LBS broth) were collected by centrifugation, washed with artificial seawater (ASW) (0.6 M NaCl, 0.1 M MgSO₄, 0.02 M CaCl₂, 0.02 M KCl, 50 mM Tris-HCl [pH 8.3] [28]), and resuspended in the appropriate medium at a density of approximately 10⁶ to 10⁷ cells/ml . During incubation under stress conditions at 30°C, aliquots were removed and spread on LBS agar plates to monitor the viability by determining the number of CFU . For survival studies under stress conditions, we used hyperosmosis (LBS medium containing 5 M NaCl), starvation (nutrient-free ASW), acidity (LBS medium titrated to pH 4.0 with HCl), UV irradiation (wavelength, 254 nm; energy, 120,000 µJ/cm²), and hydrogen peroxide (0.088 to 10 mM H₂O₂ in ASW) .

Determination of catalase activities. Cellular extracts of E . coli and various V . vulnificus strains (Table 1) were prepared in cold 50 mM potassium phosphate buffer (pH 7.0) by sonication (Vibracell; Sonics & Materials, Inc.) in ice . The amount of protein in a cell lysate was determined by the Bradford assay by using bovine serum albumin as the standard . After separation on an 8% nondenaturing polyacrylamide gel, the locations of HPI and HPII were visualized by staining the gel with a solution containing 1% K₃Fe(CN)₆ and 1% FeCl₃ (47) and compared with the locations of the corresponding enzymes of E . coli .

For the catalase assay, cell samples were obtained at various growth phases (OD₆₀₀, 0.1 to 4.2) and were resuspended in chilled catalase buffer (5 mM potassium phosphate buffer [pH 7.0], 5 mM EDTA, 10% glycerol, 25 µM phenylmethylsulfonyl fluoride) (42) and sonicated in ice . Each cellular extract was then mixed with 25 mM potassium phosphate buffer (pH 7.0) containing 5.9 mM H₂O₂, and the amount of remaining H₂O₂ in the reaction mixture was estimated by monitoring the absorbance at 240 nm at 30-s intervals for 10 min . One unit of specific activity was defined as 1 µmol of H₂O₂ degraded per min per mg of protein (42) .

Construction of katG::luxAB transcriptional fusion and measurement of expression of the katG gene. The 504-bp DNA fragment which included nucleotide positions –318 to 115 relative to the initiation codon of katG (gene VV12755 in GenBank accession no. NC_004459) was amplified by PCR by using two primers, katG-F-KpnI and katG-R-XbaI (Table 1) . The PCR product was digested with appropriate restriction enzymes (KpnI and XbaI) and inserted into luxAB-based plasmid pHK0011 (12) digested with the same enzymes . The resultant transcriptional fusion, pHL-03, was transferred into V . vulnificus cells via conjugative transfer . Overnight (16- to 18-h) cultures of the cells containing pHL-03, which exhibited the basal level of bioluminescence, were inoculated into fresh LBS medium containing 3 µg of tetracycline per ml, and the expression from the katG promoter was measured by monitoring light production in the presence of 0.006% n-decyl aldehyde by using luminometers (TD-20/20; Turners Designs) . The specific bioluminescence was calculated by normalizing the relative light units with cell mass (OD₆₀₀) .

Complementation of KPR101 with a broad-host-range vector containing V . vulnificus rpoS (pKP14) or V . vulnificus katG (pKP51). An EcoRI-HindIII DNA fragment that included the intact rpoS gene was obtained from pINE32 and cloned into the broad-host-range vector pLAFR5 (14) to obtain plasmid pKP14 . The 2,569-bp DNA fragment that included the intact katG gene was amplified by PCR by using two primers, katG-F-KpnI and katG-R-HindIII . The PCR product was digested with appropriate restriction enzymes (KpnI and HindIII) and cloned into the broad-host-range vector pRK415 (14) to obtain plasmid pKP51 . Each plasmid was introduced into the rpoS mutant by conjugative transfer, as described above .

Western analysis of ^S. Two oligonucleotides, rpoS_vv-F and rpoS_vv-R (Table 1), were used to amplify a 1,032-bp DNA fragment containing the complete sequence of the rpoS gene from the genomic DNA of V . vulnificus . BamHI and HindIII sites located at both ends of the resultant rpoS DNA were used to clone this DNA into the pQE30 expression plasmid (Qiagen) to generate plasmid pQErpoS . Recombinant ^S was overexpressed in E . coli JM109 by adding isopropylthio-ß-D-galactoside (Sigma) at a concentration of 1.0 mM and was purified by using an Ni⁺-nitrilotriacetic acid affinity column as directed by the manufacturer (Qiagen) . Polyclonal antibodies against V . vulnificus ^S were produced in a rabbit by intravenous immunization with 200 µg of the recombinant V . vulnificus ^S, and this initial immunization was followed by additional immunizations at 1 and 4 weeks . Ten days after the last injection, the blood of the immunized rabbit was collected, and its serum was used for Western blot analysis . Cell extracts of the V . vulnificus wild type and the rpoS mutant containing either pLAFR5 or pKP14 were prepared by sonication in TNT buffer (10 mM Tris-HCl [pH 8.0], 150 mM NaCl, 0.05% Tween 20) (29), and 40-µg aliquots of the extracts were fractionated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis . After transfer to a Hybond P membrane (Amersham), Western blot analysis was performed by serially incubating the filter with V . vulnificus ^S polyclonal antibodies (1:1,000 dilution) and alkaline phosphatase-conjugated rabbit anti-rat immunoglobulin G (1:1,000 dilution; Sigma) . The V . vulnificus ^S band was visualized by using the nitroblue tetrazolium-BCIP (5-bromo-4-chloro-3-indolylphosphate) system (Promega) .

Nucleotide sequence accession number. The V . vulnificus rpoS nucleotide sequence has been deposited in the GenBank database under accession number AY187681 .

 
Isolation of V . vulnificus rpoS by functional complementation. In E . coli, ^S is known to regulate the expression of several genes involved in cellular adaptation to diverse stresses . Since the ^S homologue of V . vulnificus, if there is one, may also be able to play an equivalent role in regulation of these genes, E . coli strain ZK918 containing the ^S-dependent bolA promoter::lacZ fusion (2) was utilized . Upon transformation of ZK918 with the genomic library of V . vulnificus, the bluish transformants on LB medium supplemented with X-Gal were chosen as candidates for complementing plasmids for the rpoS function . One of the plasmids, plasmid pINE32 carrying a 2,693-bp insert (Table 1), was used for further investigation .

Analysis of the pINE32 insert DNA. Sequence analysis of the insert in pINE32 revealed that it coded for the proteins of V . vulnificus homologous to NlpD, RpoS, and MutS . Although the genetic organization of the open reading frames flanking rpoS is the same as that found in other bacteria, the lengths of the intergenic spaces between nlpD and rpoS and between pcm (the upstream gene of nlpD) and nlpD were quite different from the lengths of the intergenic spaces in E . coli or Pseudomonas . This finding suggests that the regulation of rpoS expression at the transcriptional level in V . vulnificus may be different from the regulation in other organisms which have been extensively studied (20, 30, 41) . The amino acid sequence deduced from the gene homologous to rpoS, which codes for 343 amino acid residues corresponding to ca . 39.6 kDa with a pI of 4.92, was aligned with other known ^S sequences and was found to exhibit overall levels of identity of 83, 79, and 70% with the sequences of V . parahaemolyticus, V . cholerae, and E . coli, respectively . There is complete homology in subregions 2.3 and 2.4 of ^S, which are involved in promoter recognition (e.g., RpoD box and 14-mer) (4), and there is significant conservation in subregion 2.1, which is involved in core binding . The helix-turn-helix motif in subregion 3.1 and the –35 recognition region in subregion 4.2 showed relatively weak similarity .

Generation of an rpoS-deficient strain, KPR101. A major portion of the V . vulnificus rpoS gene in pINE32 was deleted by digestion with NruI and subsequent ligation . The nlpD-rpoS-mutS region with the rpoS gene deleted was transferred to a conjugative plasmid, pDM4, resulting in pKP13 . Replacement of the wild-type rpoS gene located on the chromosome of V . vulnificus AR with this plasmid was accomplished through homologous recombination . Deletion of the rpoS gene in the V . vulnificus mutant was confirmed by PCR by using primers F2 and R2 (Table 1) . A PCR analysis of a deletion of the internal region of the rpoS gene in the mutant revealed the expected size for the DNA fragment (754 bp); meanwhile, the intact rpoS gene in the wild-type produced a 1,516-bp DNA fragment (data not shown) . The resultant mutant was designated KPR101 .

Survival characteristics of KPR101. The survival of KPR101 in the exponential phase was examined when it was exposed to various stresses, including hyperosmotic conditions, starvation, an acid environment, UV irradiation, and oxidative conditions, and was compared to the survival of the wild type . In contrast to enteric bacteria (9, 19), rpoS-deficient V . vulnificus exhibited the same survival pattern in the presence of a high salt concentration (5 M NaCl) that the wild type exhibited (data not shown) . The survival of the mutant, however, was severely impaired in the presence of other stresses . For example, the abilities of the mutant to survive under starvation, acidic, and UV-irradiated conditions (6 days, 1 h, and 12 s, respectively) were estimated to be 25-, 1,300-, and 16-fold less than those of the corresponding controls, respectively (Fig . 1A C) .

 
The rpoS mutant cells in the exponential phase also showed significantly increased susceptibility to 880 µM H₂O₂; there was up to a 1,000-fold difference after 30 min of exposure (Fig . 2A) . The KPR101 cells in the stationary phase showed more resistance than the cells in the exponential phase, but the susceptibility was basically similar to the susceptibility of the wild type in the presence of various concentrations of H₂O₂ up to 10 mM (Fig . 2B) . This ^S-independent increase in H₂O₂ resistance in the stationary phase is an unusual observation, since synthesis of ^S is induced in the stationary phase in V . vulnificus (data not shown), and one of catalases (HPII) is known to be induced by ^S in E . coli (30, 37, 40) . In addition, V . vulnificus cells were generally more sensitive to H₂O₂ than other enteric bacteria were, because exposure to the concentrations of H₂O₂ used for E . coli or V . cholerae (e.g., ca . 10 mM for 30 min) resulted in survival of only 0.1 to 0.01% of the cells present initially (Fig . 2B) . Thus, it is possible that V . vulnificus may have mechanisms for oxidative stress response that are distinct from those found in E . coli, at least under the conditions which we used .

 
Characterization of the catalase of V . vulnificus. The distinct susceptibility of KPR101 to H₂O₂, especially during the exponential phase, led us to examine the innate properties of hydroperoxidase(s) in wild-type V . vulnificus . Protein extracts of the type strain of V . vulnificus (ATCC 29307) were separated on a nondenaturing polyacrylamide gel, and the bands representing hydroperoxidase activities were compared with those of a stationary-phase E . coli extract . In contrast to E . coli, which has both KatG (HPI; a multimer composed of two 80.0-kDa subunits) and KatE (HPII; a multimer composed of four 84.2-kDa subunits), only the band corresponding to HPI was visualized in both exponential- and stationary-phase V . vulnificus extracts (Fig . 3A) . The calculated molecular mass of the deduced KatG polypeptide of V . vulnificus (VV12755 in GenBank accession no. NC_004459) is estimated to be 80.4 kDa . The absence of HPII activity seemed to be common in this bacterial species, since various V . vulnificus strains exhibited only HPI activity, at least under the conditions which we tested (Fig . 3B) .

 
When the katG gene of V . vulnificus was disrupted, no hydroperoxidase band appeared (data not shown), and the missing HPI band was restored when the V . vulnificus katG gene was supplied in a multicopy plasmid (J . H . Rhee, personal communication) . The katE gene is present on chromosomal DNA of V . vulnificus (VV21473 in GenBank accession no. NC_004460), and the molecular mass of the deduced polypeptide is predicted to be 55.4 kDa . However, no apparent KatE (HPII) activity was observed under any of the conditions tested, even when we used large amounts of cellular extract (up to 200 µg of crude protein extract [data not shown]) and cellular extracts were exposed to H₂O₂ (Fig . 3A) . In addition, no transcript for katE was detected in the total RNA (30 µg) by Northern analysis with a 1,523-bp katE gene probe (data not shown) . Exposure of the exponential-phase cells to H₂O₂ resulted in the induced level of HPI found in the stationary-phase cells, which suggests that a redox-operated regulator, possibly OxyR, is involved in activating katG (46; I . Kong, A . Huelsmann, and J . D . Oliver, 102nd Gen . Meet . Am . Soc . Microbiol., poster no . K-94, 2002) .

Determination of HPI activity in the wild-type strain and KPR101. To identify the possible role of ^S in regulation of the activity of KatG, HPI activities were monitored along the growth curve (Table 2) . The HPI catalase specific activity of the wild-type strain was about 2 U during the early exponential phase (for the first 2 h of growth) and gradually decreased during the mid-exponential phase . Then it reached a maximal level, approximately 6 to 8 U, after the cells entered the late stationary phase . The activity of HPI in V . vulnificus cells during the whole growth period, except for an initiation period during the stationary phase (OD₆₀₀, 2.2 and 3.2 [Table 2]), was regulated by the presence of ^S, since the rpoS mutant contained about twofold less HPI than the wild-type strain contained . Thus, the induction of HPI at the onset of the stationary phase may depend on other regulators .

 
Similarly, the HPI catalase specific activity in KPR101 was 2 to 3 U at the onset of the stationary phase, but it did not reach the maximal level observed in the wild type (Table 2) . However, the twofold reduction in HPI activity in late-stationary-phase KPR101 compared to the activity in the wild type did not result in a difference in survival in the presence of H₂O₂ (Fig. 2B), because this amount of HPI activity (i.e., more than 2 to 3 U) might provide as much resistance to the concentrations of H₂O₂ used (up to 10 mM) as the amount in the wild type provides .

The medium used to grow KPR101 contained less HPI activity than the medium used to grow the wild type contained . No activity was detected in a cell-free medium (glucose-based ASW) which was used to grow KPR101 at the exponential phase, whereas significant HPI activity (0.38 ± 0.05 U) was found in the spent medium used for the wild type at the exponential phase . In the medium used to culture KPR101 at the stationary phase, the extracellular HPI activity (0.97 ± 0.06 U) was about 70% of the activity of the wild type (1.32 ± 0.08 U) . This suggests that the smaller amount of KatG activity in KPR101 than in the wild type was not due to increased excretion of this enzyme .

Complementation of KPR101 with a broad-host-range vector containing the V . vulnificus rpoS gene, pKP14. After pKP14, a pLAFR5-based plasmid containing the V . vulnificus rpoS gene, was added to KPR101, the expression of V . vulnificus ^S in this strain was confirmed by Western blotting by using V . vulnificus ^S-specific polyclonal antibody, which clearly showed the presence of an 39-kDa V . vulnificus ^S (Fig . 4A, inset) . The exponential-phase KPR101 culture, containing pKP14 grown in glucose-based ASW supplemented with tetracycline, was exposed to 880 µM H₂O₂, and changes in the number of CFU were monitored for 2 h . This strain was found to be resistant to H₂O₂, whereas KPR101 containing pLAFR5 was found to be sensitive to the same concentration of H₂O₂ (Fig . 4A) .

 
When the V . vulnificus rpoS gene was present in trans, apparently increased HPI activity was observed by the gel staining assay (Fig . 4B), and the increase was estimated to be about fourfold as determined by an H₂O₂ degradation kinetic study (Fig . 4C) . These results show that in the exponential phase the rpoS mutant complemented with the V . vulnificus rpoS gene exhibited both resistance to H₂O₂ and HPI activity .

Complementation of KPR101 with a broad-host-range vector containing the V . vulnificus katG gene, pKP51. If the effect of an rpoS mutation on increased sensitivity to H₂O₂ was mainly due to a lower level of HPI, KPR101 should become resistant to H₂O₂ if multiple copies of the katG gene are provided . Thus, KPR101 was complemented with pKP51, a pRK415-based plasmid containing the V . vulnificus katG gene . In the exponential phase KPR101 containing pKP51 grown in LBS medium supplemented with tetracycline exhibited much greater HPI activity (Fig . 5A) . This strain also exhibited greater resistance to 880 µM H₂O₂ than KPR101 containing pRK415 exhibited (Fig . 5B) . However, it is possible that the other gene products regulated by ^S play an important role in survival in the presence of higher concentrations of H₂O₂ than we tested . Currently, the proteins which are induced in the wild type in the exponential phase by exposure to H₂O₂ but are not induced in KPR101 in the exponential phase under the same conditions are being investigated by proteome analyses by using two-dimensional matrix-assisted laser desorption ionization—time of flight mass spectrometry .

 
Determination of katG expression in the wild type and KPR101. Since the presence of ^S apparently increases HPI activity, its role in controlling HPI was analyzed further by monitoring expression of the katG gene in the wild type and KPR101 . To do this, a luxAB-based transcriptional fusion, pHL-03 containing the promoter region of the katG gene, was constructed and transferred to both strains . In the wild-type cells, induction of the katG fusion was apparently initiated during the early exponential phase (during the first 1 to 2 h of incubation), and the level decreased to the basal level during the mid-exponential phase . A high level of expression during the initial incubation period was also observed in E . coli (8), and the HPI activity was also high at this stage of growth (Table 2) . Then induction occurred again at the onset of the stationary phase, and the level of expression reached the maximal level (about 10-fold greater than the basal level) when the cells entered the late stationary phase (Fig. 6) . This expression profile essentially parallels the pattern of catalase activity measured directly (Table 2) .

 
The katG expression in KPR101 followed the same pattern as the katG expression in the wild type, but the degrees of induction in both the early exponential and late stationary phases were significantly reduced (Fig . 6) . This pattern of V . vulnificus katG expression is quite different from the katG expression in E . coli . In E . coli, the maximal katG expression was only slightly reduced in an rpoS mutant (8), the maximal induction of katG occurred during the late exponential phase (22), and the duration of induced katG expression was not prolonged during the late stationary phase (8) . Interestingly, an HPII-deficient E . coli mutant has been reported to exhibit higher HPI activity than the parental strain exhibits (42) .

While no difference in katG expression was observed during the mid-exponential phase (Fig . 6), the estimated HPI activities in KPR101 were about 50% of those in the wild type at the same growth stage (Table 2) . This difference in activity might result from different expression during the early exponential phase . Otherwise, ^S might not directly regulate KatG at the transcriptional level, at least during the mid-exponential phase . Instead, some factors regulated by ^S are involved in increased (or sustained) activity of HPI . It is necessary to identify these factors in order to elucidate the regulatory pathways for catalase via ^S in exponential-phase V . vulnificus . The experiments in which we examined the effect of H₂O₂ on synthesis of ^S revealed a slightly increased amount of ^S in the exponential-phase cells exposed to nonlethal concentrations of H₂O₂ (data not shown) . However, additional studies are necessary to clarify whether the slightly increased amount of ^S upregulates the synthesis and/or activity of KatG during the exponential phase .

Several research groups have emphasized the importance of ^S in bacterial survival in the stationary phase and in resistance to H₂O₂ via regulation of HPII . Although it has been reported that in the stationary phase HPI is partially induced by ^S in E . coli (8, 24) and in the exponential phase some virulence genes are regulated by ^S in Salmonella dublin (5), exponential-phase induction of HPI by ^S has not been examined previously . In the present study, however, we found that in V . vulnificus this global regulator plays a role in the response to oxidative stress during the exponential phase by increasing the amount of HPI with no involvement of HPII . Investigation of the other roles of ^S in hierarchical regulatory cascades and the expression of rpoS in the presence of specific stresses is in progress .

 
This research was supported by the 21C Frontier Microbial Genomics and Applications Center Program, Ministry of Science and Technology (grant MG02-0201-004-2-1-0 to K.-H.L.), Republic of Korea .

We thank E.-K . Jeon and J . H . Lee for technical assistance, J . H . Rhee for providing a V . vulnificus katG mutant strain, H.-J . Myung for overexpression of V . vulnificus ^S, and J . K . Lee for helpful discussions .

 
* Corresponding author . Mailing address: Department of Environmental Science, Hankuk University of Foreign Studies, Wangsan-Li, Mohyun-Myun, Yongin, Kyunggi-Do 449-791, Korea . Phone: 82-31-330-4039 . Fax: 82-31-333-1696 . E-mail: khlee@san.hufs.ac.kr .

Present address: Department of Microbiology, University of Idaho, Moscow, Idaho .

1. Bang, Y . B., S . E . Lee, J . H . Rhee, and S . H . Choi. 1999 . Evidence that expression of the Vibrio vulnificus hemolysin gene is dependent on cyclic AMP receptor protein . J . Bacteriol . 181:7639-7642 .
2. Bohannon, D . E., N . Connell, J . Keener, A . Tormo, M . Espinosa-Urgel, M . M . Zambrano, and R . Kolter. 1991 . Stationary-phase-inducible "gearbox" promoters: differential effects of katF mutations and role of ⁷⁰ . J . Bacteriol . 173:4482-4492.
3. Brown, S . M., M . L . Howell, M . L . Vasil, A . J . Anderson, and D . J . Hassett. 1995 . Cloning and characterization of the katB gene of Pseudomonas aeruginosa encoding a hydrogen peroxide-inducible catalase: purification of KatB, cellular localization, and demonstration that it is essential for optimal resistance to hydrogen peroxide . J . Bacteriol . 177:6536-6544.
4. Burgess, R . R., and L . Anthony. 2001 . How sigma docks to RNA polymerase and what sigma does . Curr . Opin . Microbiol . 4:126-131.
5. El-Gedaily, A., G . Paesold, C.-Y . Chen, D . G . Guiney, and M . Krause. 1997 . Plasmid virulence gene expression induced by short-chain fatty acids in Salmonella dublin: identification of rpoS-dependent and rpoS-independent mechanisms . J . Bacteriol . 179:1409-1412.
6. Farr, S . B., and T . Kogoma. 1991 . Oxidative stress responses in Escherichia coli and Salmonella typhimurium. Microbiol . Rev . 55:561-585.
7. Faruque, S . M., M . J . Albert, and J . J . Mekalanos. 1998 . Epidemiology, genetics, and ecology of toxigenic Vibrio cholerae. Microbiol . Mol . Biol . Rev . 62:1301-1314 .
8. Gonzalez-Flecha, B., and B . Demple. 1997 . Homeostatic regulation of intracellular hydrogen peroxide concentration in aerobically growing Escherichia coli. J . Bacteriol . 179:382-388.
9. Hengge-Aronis, R. 2002 . Signal transduction and regulatory mechanisms involved in control of the ^s (RpoS) subunit of RNA polymerase . Microbiol . Mol . Biol . Rev . 66:373-395 .
10. Hollis, D . G., R . E . Weaver, C . N . Baker, and C . Thornsberry. 1976 . Halophilic Vibrio species isolated from blood cultures . J . Clin . Microbiol . 3:425-431.
11. Ichise, N., N . Morita, T . Hoshino, K . Kawasaki, I . Yumoto, and H . Okuyama. 1999 . A mechanism of resistance to hydrogen peroxide in Vibrio rumoiensis S-1 . Appl . Environ . Microbiol . 65:73-79 .
12. Jeong, H . S., K . C . Jeong, H . K . Choi, K.-J . Park, K.-H . Lee, J . H . Rhee, and S . H . Choi. 2001 . Differential expression of Vibrio vulnificus elastase gene in a growth phase-dependent manner by two different types of promoters . J . Biol . Chem . 276:13875-13880 .
13. Jeong, K . C., H . S . Jeong, J . H . Rhee, S . E . Lee, S . S . Chung, A . M . Starks, G . M . Escudero, P . A . Gulig, and S . H . Choi. 2000 . Construction and phenotypic evaluation of a Vibrio vulnificus vvpE mutant for elastolytic protease . Infect . Immun . 68:5096-5106 .
14. Keen, N . T., S . Tamaki, D . Kobayashi, and D . Trollinger. 1988 . Improved broad-host-range plasmid for DNA cloning in Gram-negative bacteria . Gene 70:191-197.
15. Klotz, M . G., G . R . Klassen, and P . C . Loewen. 1997 . Phylogenetic relationships among prokaryotic and eukaryotic catalases . Mol . Biol . Evol . 14:951-958.
16. Kolter, R., D . A . Siegele, and A . Tormo. 1993 . The stationary phase of the bacterial life cycle . Annu . Rev . Microbiol . 47:855-874.
17. Lee, S . E., S . H . Shin, S . Y . Kim, Y . R . Kim, D . H . Shin, S . S Chung, Z . H . Lee, J . Y . Lee, K . C . Jeong, S . H . Choi, and J . H . Rhee. 2000 . Vibrio vulnificus has the transmembrane transcription activator ToxRS stimulating the expression of the hemolysin gene vvhA. J . Bacteriol . 182:3405-3415 .
18. Litwin, C . M., and S . B . Calderwood. 1993 . Cloning and genetic analysis of the Vibrio vulnificus fur gene and construction of a fur mutant by in vivo marker exchange . J . Bacteriol . 175:706-715.
19. Matin, A., E . A . Auger, P . H . Blum, and J . E . Schultz. 1989 . Genetic basis of starvation survival in nondifferentiating bacteria . Annu . Rev . Microbiol . 43:293-316.
20. McCann, M . P., C . D . Fraley, and A . Matin. 1993 . The putative factor KatF is regulated posttranscriptionally during carbon starvation . J . Bacteriol . 175:2143-2149.
21. Merrell, D . S., A . D . Tischler, S . H . Lee, and A . Camilli. 2000 . Vibrio cholerae requires rpoS for efficient intestinal colonization . Infect . Immun . 68:6691-6696 .
22. Michan, C., M . Manchado, G . Dorado, and C . Pueyo. 1999 . In vivo transcription of the Escherichia coli oxyR regulon as a function of growth phase and in response to oxidative tress . J . Bacteriol . 181:2759-2764 .
23. Milton, D . L., R . O'Toole, O . Horstedt, and H . Wolf-Watz. 1996 . Flagellin A is essential for the virulence of Vibrio anguillarum. J . Bacteriol . 178:1310-1319.
24. Mukhopadhyay, S., and H . E . Schellhorn. 1994 . Induction of Escherichia coli hydroperoxidase I by acetate and other weak acids . J . Bacteriol . 176:2300-2307.
25. Mulvey, M . R., J . Switala, A . Borys, and P . C . Loewen. 1990 . Regulation of transcription of katE and katF in Escherichia coli. J . Bacteriol . 172:6713-6720.
26. Oliver, J . D. 1993 . Formation of viable but nonculturable cells, p . 239-272 . In S . Kjelleberg (ed.), Starvation in bacteria . American Society for Microbiology, Washington, D.C.
27. Oliver, J . D., F . Hite, D . McDougald, N . L . Andon, and L . M . Simpson. 1995 . Entry into, and resuscitation from, the viable but nonculturable state by Vibrio vulnificus in an estuarine environment . Appl . Environ . Microbiol . 61:2624-2630.
28. Ruby, E . G., and K . H . Nealson. 1977 . Pyruvate production and excretion by the luminous marine bacteria . Appl . Environ . Microbiol . 34:164-169.
29. Sambrook, J., and D . W . Russell. 2001 . Molecular cloning: a laboratory manual, 3rd ed . Cold Spring Harbor Laboratory Press, Cold Spring Harbor, N.Y.
30. Schellhorn, H . E., and V . L . Stones. 1992 . Regulation of katF and katE in Escherichia coli K-12 by weak acids . J . Bacteriol . 174:4769-4776.
31. Schultz, J . E., G . I . Latter, and A . Matin. 1988 . Differential regulation by cyclic AMP of starvation protein synthesis in Escherichia coli. J . Bacteriol . 170:3903-3909.
32. Seshadri, R., and J . E . Samuel. 2001 . Characterization of a stress-induced alternate sigma factor, RpoS, of Coxiella burnetii and its expression during the development cycle . Infect . Immun . 69:4874-4883 .
33. Shao, C.-P., and L.-I . Hor. 2001 . Regulation of metalloprotease gene expression in Vibrio vulnificus by a Vibrio harveyi LuxR homologue . J . Bacteriol . 183:1369-1375 .
34. Simon, R., U . Priefer, and A . Pühler. 1983 . A broad host range mobilization system for in vivo genetic engineering: transposon mutagenesis in gram negative bacteria . Bio/Technology 1:784-791.
35. Simpson, L . M., and J . D . Oliver. 1983 . Siderophore production by Vibrio vulnificus. Infect . Immun . 42:644-649.
36. Slauch, J., R . Taylor, and S . Maloy. 1997 . Survival in a cruel world: how Vibrio cholerae and Salmonella respond to an unwilling host . Genes Dev . 11:1761-1774.
37. Storz, G., and J . A . Imlay. 1999 . Oxidative stress . Curr . Opin . Microbiol . 2:188-194.
38. Strom, M . S., and R . N . Paranjpye. 2000 . Epidemiology and pathogenesis of Vibrio vulnificus. Microbes Infect . 2:177-188.
39. Suh, S.-J., L . Silo-Suh, D . W . Woods, D . J . Hassett, S . E . H . West, and D . E . Ohman. 1999 . Effect of rpoS mutation on the stress response and expression of virulence factors in Pseudomonas aeruginosa. J . Bacteriol . 181:3890-3897 .
40. Switala, J., J . O . O'Neil, and P . C . Loewen. 1999 . Catalase HPII from Escherichia coli exhibits enhanced resistance to denaturation . Biochemistry 38:3895-3901.
41. Venturi, V. 2003 . Control of rpoS transcription in Escherichia coli and Pseudomonas: why so different? Mol . Microbiol . 49:1-9.
42. Visick, J . E., and S . Clarke. 1997 . RpoS- and OxyR-independent induction of HPI catalase at stationary phase in Escherichia coli and identification of rpoS mutations in common laboratory strains . J . Bacteriol . 179:4158-4163.
43. Visick, K . L., and M . J . McFall-Ngai. 2000 . An exclusive contract: specificity in the Vibrio fischeri-Euprymna scolopes partnership . J . Bacteriol . 182:1779-1787.
44. Visick, K . L., and E . G . Ruby. 1998 . The periplasmic, group III catalase of Vibrio fischeri is required for normal symbiotic competence and is induced both by oxidative stress and by approach to stationary phase . J . Bacteriol . 180:2087-2092 .
45. Vivas, E . I., and H . Goodrich-Blair. 2001 . Xenorhabdus nematophilus as a model for host-bacterium interactions: rpoS is necessary for mutualism with nematodes . J . Bacteriol . 183:4687-4693 .
46. Waldron, D . E., P . Owen, and C . J . Dorman. 2002 . Competitive interaction of the OxyR DNA-binding protein and the Dam methylase at the antigen 43 gene regulatory region in Escherichia coli. Mol . Microbiol . 44:509-520.
47. Wayne, L . G., and G . A . Diaz. 1986 . A double staining method for differentiation between two classes of mycobacterial catalase in polyacrylamide electrophoresis gels . Anal . Biochem . 157:89-92.
48. Wright, A . C., J . G . Morris, Jr., D . R . Maneval, Jr., K . Richardson, and J . B . Baker. 1985 . Cloning of the cytotoxin-hemolysin gene of Vibrio vulnificus. Infect . Immun . 50:922-924.
49. Yanisch-Perron, C., J . Vieira, and J . Messing. 1985 . Improved M13 phage cloning vectors and host strains: nucleotide sequences of the M13mp18 and pUC19 vectors . Gene 33:103-119.
50. Yildiz, F . H., and G . K . Schoolnik. 1998 . Role of rpoS in stress survival and virulence of Vibrio cholerae. J . Bacteriol . 180:773-784 .
51. Yumoto, I., D . Ichihashi, H . Iwata, A . Istokovics, N . Ichise, H . Matsuyama, H . Okuyama, and K . Kawasaki. 2000 . Purification and characterization of a catalase from the facultatively psychrophilic bacterium Vibrio rumoiensis S-1^T exhibiting high catalase activity . J . Bacteriol . 182:1903-1909 .

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