Pseudomonas aeruginosa IscR-Regulated Ferredoxin NADP(+) Reductase Gene (fprB) Functions in Iron-Sulfur Cluster Biogenesis and Multiple Stress Response

Abstract

P. aeruginosa (PAO1) has two putative genes encoding ferredoxin NADP(+) reductases, denoted fprA and fprB. Here, the regulation of fprB expression and the protein’s physiological roles in [4Fe-4S] cluster biogenesis and stress protection are characterized. The fprB mutant has defects in [4Fe-4S] cluster biogenesis, as shown by reduced activities of [4Fe-4S] cluster-containing enzymes. Inactivation of the gene resulted in increased sensitivity to oxidative, thiol, osmotic and metal stresses compared with the PAO1 wild type. The increased sensitivity could be partially or completely suppressed by high expression of genes from the isc operon, which are involved in [Fe-S] cluster biogenesis, indicating that stress sensitivity in the fprB mutant is partially caused by a reduction in levels of [4Fe-4S] clusters. The pattern and regulation of fprB expression are in agreement with the gene physiological roles; fprB expression was highly induced by redox cycling drugs and diamide and was moderately induced by peroxides, an iron chelator and salt stress. The stress-induced expression of fprB was abolished by a deletion of the iscR gene. An IscR DNA-binding site close to fprB promoter elements was identified and confirmed by specific binding of purified IscR. Analysis of the regulation of fprB expression supports the role of IscR in directly regulating fprB transcription as a transcription activator. The combination of IscR-regulated expression of fprB and the fprB roles in response to multiple stressors emphasizes the importance of [Fe-S] cluster homeostasis in both gene regulation and stress protection.

Introduction

Ferredoxin NADP(+) reductase (Fpr) is a flavin adenine dinucleotide (FAD)-containing oxidoreductase enzyme. It catalyzes reversible electron transfer between NADPH and electron carrier [Fe-S] proteins such as ferredoxin and flavodoxin [1, 2]. During photosynthesis, Fpr-ferredoxin complexes facilitate electron transfer from the Photosystem I to NADP⁺, generating NADPH for CO₂ assimilation [3]. Bacterial Fprs also have ferric reductase activity [4]. Fpr also catalyzes a diaphorase reaction, which is an irreversible oxidation of NADPH in the presence of different electron acceptors such as ferricyanide, complexed transition metals, substituted phenols, nitro-derivatives, tetrazolium salts, viologens, quinones, and cytochromes [5].

Fprs are widely distributed in organisms ranging from bacteria to eukaryotes. These enzymes are divided into two main classes based on the structure, a plastid class and a bacterial class [6]. The plastid Fprs are found in photosynthetic organisms. Bacterial Fprs can be further subdivided into two subclasses. Subclass I Fprs have structures similar to that of the prototype Azotobacter vinelandii Fpr, while the structures of subclass II Fprs are homologous to that of the Escherichia coli Fpr [6, 7]. Among bacterial Fprs, subclass I Fpr typically contain less ferredoxin NADP(+) reductase catalytic efficiency than subclass II Fpr [4], and some Fprs have ferric reductase activity [4, 8]. The physiological role of Fpr in bacteria is unclear, though it has been shown to function in the bacterial oxidative stress response [4, 8]. Inactivation of subclass II fpr in E. coli increases sensitivity to paraquat (PQ), a superoxide-generating agent [8]. Increased expression of Fpr is associated with enhanced survival rate under superoxide stress [9]. The expression of fpr in E. coli and Salmonella is regulated by SoxRS proteins, transcriptional regulators that sense and respond to superoxide stress [9]. Moreover, Pseudomonas putida contains two Fprs, namely, fprA and fprB. The expression of fprA (encoding subclass I Fpr) is induced in response to superoxide stress and is regulated by FinR, a LysR-type transcriptional regulator [10]. Both FprA and FinR have important roles in cellular defense against stress due to superoxide and ferrous iron depletion [10–12]. The expression of fprB (encoding subclass II Fpr) is not affected by exposure to oxidants but is induced by osmotic stress [13]. The disruption of fprB in P. putida exhibits growth defects under high osmotic stress conditions and slower rate of recovery of oxidatively damaged aconitase (an [4Fe-4S]-containing enzyme) activity than that of the wild type [13].

Recently, Fpr has been shown to have roles in [Fe-S] cluster biogenesis in E. coli. One of the products from Fpr-catalyzed reactions is a reduced ferredoxin that is involved in [4Fe-4S] cluster biosynthesis [14]. Hence, the activities of [4Fe-4S] cluster-containing enzymes such as aconitase [15] and succinate dehydrogenase [16] and [4Fe-4S] transcription regulators such as an auto regulated anr that activates transcription of nitrate reductase genes such as narG [17–19] could be modulated by the availability of [4Fe-4S] clusters.

Pseudomonas aeruginosa is an opportunistic human pathogen that can thrive in harsh environments such as high temperature, high salt concentration and toxic chemicals. It is highly resistant to various chemical agents, such as antiseptics and several antibiotics. P. aeruginosa has several means of counteracting stressful conditions, including oxidative stress generated by innate immune cells or the environment. These factors are thought to contribute to bacterial virulence during the infection process [12]. The function of Fpr in P. aeruginosa is poorly understood. This bacterium contains two putative ferredoxin NADP(+) reductases: one Fpr is a member of bacterial subclass I and is denoted FprA (PA3397), and the other Fpr is a member of bacterial subclass II, which is named FprB (PA4615). Recently, FprB was proposed to promote Fenton chemistry in P. aeruginosa cells treated with oxidative stress-producing antibiotics via its ferric reductase activity [4, 12]. The fprB mutant displayed enhanced resistance to ampicillin, norfloxacin and gentamicin [12]. P. aeruginosa FprA can function as an electron donor to ferritin-like molecules, such as heme-binding bacterioferritins (Bfr) and non-heme-binding bacterial ferritins (Ftn), leading to release of the iron stored by these ferritins into the cytoplasm [20]. Under iron starvation, however, FprA is an electron donor to heme oxygenase, an enzyme involved in heme metabolism [21].

In this study, the physiological function of fprB in P. aeruginosa was evaluated through phenotypic analysis of the mutant. Our data indicated that fprB has defects in [Fe-S] cluster biogenesis and that Fpr activity is required for survival under oxidative, osmotic, and metal stresses. Unlike other bacteria, the expression of fprB is controlled by IscR, a global transcriptional regulator of genes involved in [Fe-S] cluster biogenesis and stress responses.

Results and Discussion

PAO1 fprB gene and transcription organization

Analysis of the P. aeruginosa PAO1 genome database [22] identified two genes, fprA (PA3397) and fprB (PA4615), encoding putative ferredoxin NADP(+) reductase similar to that of A. vinelandii and P. putida genomes. P. aeruginosa FprA shares low (33.7%) amino acid identity with FprB (S1 Fig). P. aeruginosa FprB, a 285-amino acid protein, shares high amino acid identity with FprB from P. putida (82.9%) [13] and A. vinelandii (68.2%) [23] (Fig 1A), while it shares 36.7% identity with E. coli Fpr [8]. The major differences between Fpr sub-classes I and II are found in the C-terminal region [6]. The signature amino acid residues for Fpr sub-class II, which include the tyrosine-247 [24] and tryptophan-248 residues of E. coli Fpr [6], are conserved in P. aeruginosa FprB (Fig 1A). Thus, similar to P. putida FprB, the P. aeruginosa FprB belongs to subclass II of bacterial ferredoxin NADP(+) reductases.

Fig 1. Multiple amino acid sequence alignment and gene organization of P. aeruginosa fprB.

(A) Alignment of P. aeruginosa FprB with other characterized bacterial FprB enzymes (Ppu, P. putida; Avn, A. vinelandii; and Ecl, E. coli ATCC 8739) was performed using the CLUSTALW program [57]. Black (YW) and light gray (RAYS) boxes indicate the subclass II signature amino acid and the FAD-binding domain, respectively. The asterisk, colon, and period symbols indicate identical residues, conserved substitutions, and semi-conserved substitutions, respectively. Number indicates percent identity of the aligned protein with that of P. aeruginosa. (B) Gene organization at the fprB locus among Pseudomonas spp. fnr and fnr-2, fprB-homologous genes; katB and katE, catalase genes; mscL, gene encoding large conductance mechanosensitive channel; dctP, gene encoding propable periplasmic C4-dicarboxylate binding-protein; rsmC, gene encoding propable 16S RNA G1207 methylase; luxR, LuxR family DNA-binding transcriptional regulator gene; radA, gene encoding propable DNA repair protein; non-labelled, gene with unknown annotation.

The locations of fprB in genomes of different Pseudomonas species are varied. In most Pseudomonas spp., including P. putida, P. fluorescens, and P. entomophila, fprB is located between mscL, encoding a large conductance mechano-sensitive channel, and an open reading frame (ORF) encoding a homolog of the LuxR transcription regulator (Fig 1B). Nevertheless, the role of this LuxR family of transcription regulators in regulation of fprB in P. putida is unclear [13]. In P. syringae genome, a gene encoding putative transposase was inserted between fprB-homolog (fnr-2) and luxR (Fig 1B). Whereas, in P. aeruginosa strains such as PAO1 and PA14, fprB is located between mscL (PA4614) and PA4616, encoding a probable C4-dicarboxylate-binding protein (Fig 1B). Nonetheless, analysis of different isolates of P. aeruginosa shows significant variation in the genomic location of fprB. For example, P. aeruginosa PA7 genome contains three unknown open reading frames inserted between fprB and mscL genes (Fig 1B). Our Northern blot analysis results (in the expression analysis section) indicated that PAO1 fprB is transcribed as a monocistronic mRNA.

Expression analysis of fprB

P. aeruginosa FprB might has important roles in maintaining functional levels of [4Fe-4S] clusters. The regulation of its expression is therefore also likely to be important, especially during stressful growth conditions. The fprB expression profile was determined using end-point and real-time RT-PCR. Initially, the expression of fprB was monitored throughout all phases of bacterial growth, and no significant changes in fprB expression levels were observed during different growth phases (data not shown). Oxidative stress is known to affect the balance of [Fe-S] clusters, and hence, fprB expression levels in response to sources of oxidative stress were determined. Exposure of PAO1 to redox cyclers such as PB (0.5 mM), PQ (0.5 mM) and MD (0.5 mM) induced fprB expression at levels that ranged from 4- to 14-fold increases over the uninduced levels (Fig 2A). The effects of exposure to various peroxides were also investigated. Exposure to H₂O₂ (1 mM) produced less than a 2-fold induction, while treatment with organic hydroperoxides (tBH, 1 mM and CHP, 1 mM) induced 6- to 8.5-fold increases, respectively. DM (1 mM) induced a 14-fold increase in fprB expression (Fig 2A). Moreover, growth under low intracellular iron conditions (via addition of DIPY, 1 mM) also produced a low level (3-fold) of induction of gene expression (Fig 2A). Osmotic stress (excess NaCl or KCl) induced 2-3-fold increases in fprB expression (Fig 2A). The fprB expression profile clearly shows that treatment with redox cycling compounds and an electrophile highly induced expression levels (over 10-fold), while organic hydroperoxides (H₂O₂), low iron and osmotic stress resulted in moderate (6-8-fold) to low levels (2-3-fold) induction of expression. The stress-induced expression profile of P. aeruginosa fprB was unlike previously observed patterns in P. putida, where fprB expression was inducible by osmotic stress conditions but not by oxidative stress conditions [13]. The expression pattern of P. aeruginosa fprB supports its role in oxidative, osmotic and metal stress responses. Under these conditions, there is a higher demand for [Fe-S] cluster biogenesis and cluster repair, hence the corresponding increase in fprB expression. The induction of fprB expression by iron depletion also supports the requirement of FprB for [Fe-S] cluster biogenesis [21, 25].

Fig 2. Expression profile and characterization of fprB promoter.

(A) Real-time RT-PCR analysis of fprB expression. The PAO1 cultures were induced with 1 mM H₂O₂, 1 mM CHP, 1 mM tBH, 1 mM DM, 0.5 mM PB, 0.5 mM PQ, 0.5 mM MD, 1 mM DIPY, 5 mM NaCl or 5 mM KCl for 15 min prior to RNA preparation and real-time RT-PCR analysis as described in the experimental procedures. The data shown are the means and SD of three independent experiments. (B) Promoter characterization using primer extension assay. Reverse transcription was performed using ³²P-labeled BT3552 primer and RNA extracted from PAO1 cultured under uninduced (UN) conditions or 0.5 mM PB. The extension products were separated on an 8% acrylamide-7 M urea sequencing gel. G, A, T, C represent the DNA sequence ladder prepared using a sequencing kit (Epicentre) with ³²P-labeled primer and the putative fprB promoter fragment as template. The arrowhead points to the transcription start site (+1). The putative -10 and -35 elements are underlined. The consensus sequence of the E. coli IscR binding site is aligned above the sequence line in corresponding letters, and the homologous bases are marked by asterisks. The mutagenized bases (from GCC to TTT) in the putative IscR binding motif are shown below the sequence line.

fprB is regulated by IscR

The pattern of fprB expression in response to redox cycling agents and peroxides suggests that it could be regulated by a global superoxide–peroxide stress sensor and transcription regulator. The analysis of fprB promoter and transcription-regulator binding motifs could reveal information about the mode of regulation of the gene. Primer extension experiments were carried out to determine the 5’ end of fprB transcripts from RNA samples isolated from uninduced and PB-treated cultures. The primer extension product in both RNA samples was mapped to a G residue located 21-bp upstream of the fprB start codon (ATG) (Fig 2B). The fprB promoter motifs at the -35 and -10 regions were deduced from the transcription start site as TGTTTC and GACACT, respectively, separated by 17 nucleotides. Primer extension results also confirmed the real-time RT-PCR results that PB (0.5 mM) is a potent inducer of fprB expression, as shown by over 10-fold increase in the amount of primer extension product (Fig 2B). The data also suggest that the observed induction by PB is likely due to an increase in transcription of the gene from its promoter.

E. coli fpr (an fprB homolog) is a member of the SoxRS regulon [1]. The P. aeruginosa SoxR paradigm is different from the E. coli SoxR paradigm, in that P. aeruginosa SoxR directly regulates its target genes [26]. SoxR-regulated genes share conserved SoxR boxes located between promoter elements in a diverse group of bacteria [27, 28]. No putative SoxR binding site (CCTCAAGtttgCTTGAGG) [29] could be identified near the fprB promoter region, suggesting that SoxR does not participate in the regulation of fprB.

In P. aeruginosa, FinR, IscR, OxyR and SoxR have been shown to be sensors of superoxide-peroxide stresses [29–32]. In an attempt to identify the transcriptional regulator responsible for the regulation of P. aeruginosa fprB, expression analysis was repeated in PAO1, finR, iscR, oxyR and soxR mutants cultured in medium with and without PB. The expression of genes under the regulation of these genes is known to be highly induced upon challenge with redox cycling drugs [29–32]. End-point RT-PCR analysis revealed that PB-induced expression of fprB was presented at similar levels to PAO1 in finR, oxyR, soxR mutants, indicating that these regulators were not responsible for the PB-inducible expression of fprB (Fig 3A). In contrast, PB-induction of fprB expression was abolished in the ΔiscR mutant and was restored in the ΔiscR mutant complemented with a pIscR plasmid (Fig 3B and 3C). Similarly, the induction of fprB expression by other oxidants (H₂O₂, CHP, DM) and DIPY treatments were also abolished in the ΔiscR mutant (Fig 3C). The induction of fprB by these oxidants in the ΔiscR mutant could be restored in the ΔiscR/pIscR strain (Fig 3C). Northern blot analysis of fprB expression was performed on RNA samples purified from PAO1/pBBR, the ΔiscR/pBBR mutant and the complemented ΔiscR mutant (ΔiscR/pIscR) [32, 33] cultured with and without PB. The Northern blot results clearly show that PB highly induces fprB expression in PAO1 and that this PB induction of gene expression was abolished in the ΔiscR mutant, confirming the RT-PCR results (Fig 3B). The PB induction of fprB in the ΔiscR mutant could be restored in the complemented ΔiscR/pIscR strain (Fig 3B). The results indicate that IscR is the transcription regulator responsible for oxidant-inducible expression of fprB.

Fig 3. End-point RT-PCR and Northern blot analyses of fprB expression in P. aeruginosa strains.

(A) The fprB expression profiles in PAO1, ΔiscR, oxyR, finR, and soxR mutants were determined using end-point RT-PCR. Exponential cells were grown at 37°C under uninduced (UN) or induced conditions with 0.5 mM plumbagin (PB) for 15 min. (B) The fprB expression profiles in PAO1 harboring empty vector (PAO1/pBBR), ΔiscR mutant harboring empty vector (ΔiscR /pBBR), and the complemented ΔiscR mutant (ΔiscR mutant/pIscR) were analyzed using Northern blot. Bacteria were cultured under uninduced (UN) or induced conditions with 0.5 mM PB. (C) The fprB expression profiles in PAO1/pBBR, ΔiscR /pBBR, ΔiscR mutant/pIscR in response to reagents (i.e., 0.25 mM PB, 1 mM H₂O₂, 1 mM CHP, 1 mM DM, 1 mM DIPY, and 0.25 M NaCl) were determined using end-point RT-PCR. All data presented in this figure were representatives of triple biologically independent replications and the number indicated above or below each band represents the fold change in band intensity relative to a level of the uninduced culture of PAO1/pBBR, determined using densitometric analysis.

Further analysis of fprB expression data revealed that IscR is a transcription activator of fprB. Northern blot analysis of fprB expression showed that the basal, uninduced level of fprB expression in the ΔiscR mutant was 3.2-fold lower than the level in PAO1 (Fig 3B) and that in a complemented ΔiscR/pIscR strain, fprB was expressed at a higher (2.82-fold) level than the level in PAO1 (Fig 3B). The PB-induced level in the complemented strains (ΔiscR/pIscR) was also increased slightly (69%) over the induced levels in PAO1 (Fig 3B). Similar patterns of fprB expression in ΔiscR mutant and the complemented strains were observed using end-point RT-PCR analysis (Fig 3A and 3C). These data suggest that IscR acts as a transcriptional activator of fprB and regulates gene expression in response to redox cycling drugs. Moreover, fprB is the first gene in Pseudomonas that is shown to be activated by IscR.

The are two types of IscR binding site namely type I and type II, these sites are bound differentially by holo-IscR and apo-IscR and either repress or activate target gene expression [34, 35]. A search for an IscR box near the fprB promoter revealed a putative IscR-binding site with the sequence 5’ATAGCCACAAGCCTTGCGGGTGTTTC3’ located adjacent to the putative -35 region of the promoter (Fig 2B). This sequence box shares 78% identity with the type-II E. coli IscR binding motif (AWARCCCYTSNGTTTGMNGKKKTKWA) while it shares 44% and 52% identities with the PAO1 IscR binding motif (ATAGTTGACCNATTTTCTCGGGNAA) [32] and the type-I E. coli IscR binding motif (ATASYYGACTRWWWYAGTCRRSTAT) [34], respectively. This result supports the direct regulation of fprB by IscR and enhances a possibility that IscR binds this putative box near the fprB promoter as the type-II binding manner. The regulation of fprB by IscR was further investigated. A gel mobility shift assay was conducted using purified P. aeruginosa IscR protein with a C-terminal 6×His tag [33] and a 184-bp DNA fragment spanning the fprB regulatory region. The results demonstrated that IscR binds specifically to the identified fprB regulatory DNA fragment (Fig 4A). Excess unlabeled probe (UP), but not heterologous DNA (HD), could compete with the labeled probe in the IscR-binding complex formation. No binding complexes were detected when excess unrelated protein was added to the labeled probe instead of purified IscR in a binding reaction (Fig 4A). To assess the role of the putative IscR-binding site of the fprB promoter, PCR-based site-directed mutagenesis of the putative IscR-binding motif was performed using the fprB promoter fragment as a template. The highly conserved bases GCC of IscR binding motif of E. coli [34] in the putative IscR binding sequence 5’ATAGCCACAAGCCTTGCGGGTGTTTC3’ were mutated to TTT. The gel mobility shift experiments were performed using mutated fprB promoter, where the GCC sequence in the putative type-II IscR binding site was replaced with TTT. As shown in Fig 4B, no shift complexes were observed, indicating that mutagenesis of the putative IscR binding sequence abolished the binding ability of purified IscR. These results support the hypothesis that IscR directly binds to the fprB promoter at the proposed IscR binding site and regulates fprB expression. This is the first report of a homologous sequence of type-II IscR-binding site in P. aeruginosa genome. In E. coli, [2Fe-2S] IscR binds to both types of binding motifs, whereas apo-IscR binds to type-II motifs [36]. Spectral analysis of purified IscR used in this study had roughly 50% presence of [Fe-S] cluster [22]. Hence it was not possible to differentiate the specific protein type that binds to this proposed box near the P. aeruginosa fprB promoter. However, the type-II IscR-binding mechanism in P. aeruginosa is under investigation.

Fig 4. Gel mobility shift assay.

Purified protein preparation and protein-DNA binding assay were performed as described in the experimental procedures. The gel mobility shift assay was performed using the ³²P-labeled native (A) and mutagenic (B) fprB promoter fragment and increasing concentrations of purified IscR. UP and HD represent the addition of 1 μg unlabeled iscR promoter and 2.5 μg of heterologous DNA (pUC18 plasmid), respectively, to the binding reaction mixtures containing 3.0 μM IscR. F and B indicate free and bound probes, respectively. The data presented was a representative of three biologically independent experiments.

The regulation of fprB by IscR, an important regulator of Fe-S biogenesis and stress response, illustrates the importance of co-ordination between the gene regulation and physiological roles in the stress response. IscR negatively auto-regulates the isc operon and positively regulates fprB. Thus, the levels of IscR are important in determining the expression levels of the genes that balance [Fe-S] cluster availability and the overall ability of cells to cope with multiple stresses. E. coli apo-IscR binds type-II sites on the suf operon promoter and promotes the Fe-S biogenesis under stress conditions [34]. However, no homologues of the complete suf operon could be identified in the PAO1 genome [22] suggesting that FprB involves in the Fe-S biogenesis through the ISC system. Under low iron and oxidative stress conditions, levels of [Fe-S] cluster decreased leading increased levels of apo-IscR in the cell. This results in depression of isc-operon and increased concentrations of IscR leading to activation of fprB in order to increase the [Fe-S] cluster biogenesis.

Inactivation of fprB diminishes the activities of [Fe-S] cluster-containing enzymes

Here, we assessed the effect of fprB inactivation on the overall [Fe-S] cluster balance of the cell. The status of [Fe-S] clusters was assessed in the mutant and a parental strain. First the status of [4Fe-4S] was assessed by determining the activity levels of the [Fe-S] cluster-containing enzymes aconitase and succinate dehydrogenase (Sdh) in the fprB mutant and PAO1 [15, 16]. In addition, the relative expression of [4Fe-4S] cluster containing transcription regulator anr and one of its target gene narG [17–19] was monitored in the fprB mutant and a parental strain. The results of enzyme assays indicated that the activities of both aconitase and Sdh were reduced by approximately 50% in the fprB mutant relative to the PAO1 wild type under normal growth condition (Fig 5A). This reduction in the mutant enzyme activities could be fully complemented to wild-type levels by pFprB, an expression vector containing functional fprB (Fig 5A). In addition, the relative expression of anr and narG were reduced by 50 to 70% in the fprB mutant compared to the PAO1 strain (Fig 5B). The reduction in transcription activities of these genes in the mutant could be complemented by pFprB to PAO1 levels (Fig 5B). Moreover, expression of fprB from the expression vector resulted in two to three fold increased in the relative expression of narG over PAO1 levels (Fig 5B).

Fig 5. Iron-sulfur cluster-containing protein activities.

(A) Aconitase and succinate dehydrogenase (Sdh) activities in P. aeruginosa PAO1 and fprB mutant harboring empty vector (pBBR), pFprB, or pISC strains under normal growth condition were measured. Cell culture conditions, protein preparation and enzymatic activity assays were performed as described in the experimental procedures. The data shown are means and SD of triple biologically independent replications. The asterisk indicates a statistically significant difference (P < 0.01) compared with the PAO1/pBBR strain and pBBR referred as an empty vector control. (B) Real-time RT-PCR analysis of anr, narG, soxR and PA2274 in indicated P. aeruginosa strains cultivated under normal growth condition. RNA isolation and real-time RT-PCR were performed as described in the experimental procedures. The data shown are means and SD of three independent experiments. The asterisk indicates a statistically significant difference (P < 0.01) compared to those of the PAO1/pBBR strain.

To test whether decreases in these enzymes’ activities were resulted from the lack of active cofactor [4Fe-4S] cluster or not, pISC, an expression vector containing functional iscASU-hscBA-fdx2-iscX (genes in the P. aeruginosa isc-operon encoding necessary machineries for [Fe-S] cluster biogenesis), was transformed into the mutant and the enzymatic activities and transcription activities of the genes were monitored in these strains. Fig 5A showed that the fprB mutant harboring pISC exhibited an approximately 85% of aconitase and Sdh activities relative to the PAO1 wild type levels and has similar level of these enzymatic activities as the fprB mutant harboring pFprB. The reduction in transcription levels of anr and narG in the mutant was complemented to PAO1 levels in fprB/pISC strain (Fig 5B).

Subsequently, the status of [2Fe-2S] clusters in the mutant was determined by measuring the expression of soxR mRNA (encoding a [2Fe-2S] cluster-containing transcriptional regulator) and its target gene PA2274 by real-time RT-PCR. The data show that fprB inactivation has no effect on expression levels of an auto-regulated soxR or the SoxR-targeted gene, PA2274 relative to wild type (Fig 5B). The similar functionality of [2Fe-2S] cluster-containing proteins in the mutant and PAO1 suggests that FprB may not be involved in the maintenance of [2Fe-2S] cluster status and its inactivation does not significantly alter the physiological levels of [2Fe-2S] clusters.

The results suggest that FprB could be involved in [4Fe-4S] cluster biogenesis pathway and required for full activity of [4Fe-4S] containing enzymes and transcription regulators. FprB is catalyzed the reaction leading to formation of reduced ferredoxin, a key electron donor in the biogenesis of [4Fe-4S] cluster from [2Fe-2S] cluster [14]. Inactivation of FprB leads to decrease [4Fe-4S] cluster biogenesis, resulting in an overall decrease in the functional levels of [4Fe-4S] cluster, reflected in the observed activity reductions in aconitase and Sdh. The reduced transcription activities of [4Fe-4S] cluster-containing transcription regulator anr and its target gene narG further supported the role of fprB in [4Fe-4S] cluster biogenesis. Recently, E. coli ferredoxin, encoded by fdx2 in an isc-operon, functions in conjunction with Fpr and NADPH to transfer electrons to promote [Fe–S] cluster biogenesis [14]. The results support the notion that FprB has important role in the [4Fe–4S] cluster biogenesis. In addition, it has been proposed that P. putida FprB has the ability to repair damaged [4Fe-4S] clusters [13]. Thus, in the mutant, reduced cluster repair could further reduce the physiological, functioning levels of [4Fe-4S] cluster and potentiated the sensitivity to stresses. The mechanisms of P. aeruginosa FprB for repairing [Fe-S] clusters are under investigating.

The physiological role of fprB in the oxidative stress response

The physiological role of FprB in protection against oxidative stress was investigated using an fprB mutant and a plate sensitivity assay and exposure to various oxidative stress conditions. The fprB mutant was 10²- and 10-fold more sensitive to treatment with hydrogen peroxide (H₂O₂, 0.5 mM) and organic hydroperoxides (cumene hydroperoxide [CHP], 1.6 mM), respectively (Fig 6). The mutant was highly sensitive to treatment with redox cycling/superoxide generating-compounds PQ (200 μM), menadione (MD, 4 mM), and plumbagin (PB, 1 mM), which caused over 10⁴-fold reduction in survival percentage compared to PAO1 (Fig 6). Additionally, the mutant was 10⁴-fold more susceptible to a thiol-depleting agent diamide (DM, 13 mM) than PAO1 (Fig 6). The resistance of the mutant to other oxidative and nitrosative stresses was then measured, including a strong oxidant, sodium hypochlorite (NaOCl), and a generator of nitrosative stress, acidified sodium nitrite (NaNO₂). The results showed that the fprB mutant was over 10³- and 10²-fold more sensitive to treatments with either 0.045% NaOCl or 50 mM NaNO₂ pH 5.0, respectively, than PAO1 (Fig 6). The observed phenotypes of the fprB mutant are different from those of the closely related P. putida fprB mutant, which shows no alteration in sensitivity to PQ-induced oxidative stress [13]. However, fpr inactivation in E. coli does result in increased sensitivity to oxidative and nitrosative stress [1]. Overall, the results indicate that in P. aeruginosa, FprB has a crucial role in bacterial survival under oxidative stress and nitrosative stress conditions.

Fig 6. Determination of oxidant resistance levels of P. aeruginosa strains.

The oxidant resistance levels in P. aeruginosa PAO1 and fprB mutants that harbored either empty vector (pBBR), pFprB (for fprB expression), or pISC (for expression of the functional isc operon without iscR). The resistance levels against NaOCl (0.045%) and NaNO₂ (pH 5.0, 50 μM) were determined using a bacterial killing assay while those against other oxidants i.e., H₂O₂ (0.5 mM), cumene hydroperoxide (CHP, 1.6 M), diamide (DM, 13 mM), paraquat (PQ, 200 μM), menadione (MD, 4 mM), and plumbagin (PB, 1 mM) were performed using a plate sensitivity assay as described in the experimental procedures. The data shown are means and SD of percent survival at 18 h incubation from three independent experiments. The asterisk indicates a statistically significant difference (P < 0.01) between the two indicated strains.

Inactivation of fprB showed varying degrees of sensitivity increases to different stresses tested. The nature of these stresses was diverse, and it is likely that the sensitivity arose from a general defect of cell function. Our observations showed that the fprB mutant had reduced activities of [4Fe-4S] cluster-containing enzymes and transcription factor (Fig 5). The reduced activities of these [4Fe-4S] clusters-containing proteins could be restored fully by expression of fprB and partially by pISC. Hence, the defect in [Fe-S] cluster biogenesis is possibly responsible for the increased sensitivity to multiple stresses in the fprB mutant. Experiments were performed to test whether the mutant phenotypes of increased sensitivity to multiple oxidative stresses result from a reduced availability of [Fe-S] supply for cellular activities. We tested whether increasing levels of [Fe-S] cluster biogenesis genes could compensate for the lack of FprB in protecting the bacteria against oxidants was performed by transforming pISC into the fprB mutant. This allows direct determination of the roles [Fe-S] biogenesis in alleviating oxidant sensitivity of the fprB mutant. In E. coli, a small regulatory non-coding RNA RyhB binds to the second cistron of the iscRSUA mRNA and promotes the cleavage of the downstream iscSUA transcript but no putative ryhB or P. aeruginosa sRNA prrF (a functional ryhB analogue) binding motifs were identified between the iscR and iscS intergenic sequences of P. aeruginosa PAO1. The sensitivity levels were measured in the fprB mutant and PAO1 strains harboring either pISC, pFprB or an empty vector control. As expected, expression of fprB from a vector (fprB/pFprB) fully complemented all oxidant-sensitive phenotypes of the mutant and restored sensitivity levels to those attained in PAO1 (Fig 6). This experiment confirmed that the oxidant-sensitive phenotype arose directly from a lack of FprB. Similarly, the oxidants could be divided into three groups based on their effects on the sensitivity levels of fprB-harboring pISC (fprB/pISC) strain. The first group of oxidants, including an organic hydroperoxide (CHP) and an electrophile (DM), produced similar levels of sensitivity in fprB/pISC and control strains (Fig 6). Treatment of fprB/pISC with the second group of oxidants, including NaOCl, NaNO₂, and H₂O₂, produced an intermediate level of protection, lower than the resistance of PAO1 but higher than that of the fprB mutant (Fig 6). The presence of pISC fully protected fprB mutant from MD, PQ and PB treatments, allowing resistance of mutant to reach the level attained by PAO1 wild type (Fig 6).

It has been suggested that P. putida FprB promotes Fenton chemistry by iron mobilization from storage proteins and by ferric reductase activity, which generates ferrous ions from ferric ions in the presence of H₂O₂, leading to hydroxyl radical production and ultimately contributing to cell death [12]. If iron mobilization and ferric reductase activities by FprB in P. aeruginosa have major roles in the oxidative stress response, then inactivation of fprB should lead to increased resistance to H₂O₂. On the contrary, the P. aeruginosa fprB mutant was more susceptible to H₂O₂ treatment, suggesting that iron mobilization and ferric reductase activity are not responsible for the fprB mutant phenotype. Alternatively, Fpr may use NADPH to generate active peroxide scavengers that function in the detoxification of H₂O₂ and CHP [37]. Accordingly, fprB inactivation led to increased sensitivity to peroxides. Increased sensitivity to nitrosative stress (acidified nitrite) of the P. aeruginosa fprB mutant is not unexpected. Under acid condition, nitrite is protonated to produce HNO₂ that would undergo dismutation, generating nitric oxide radical (NO) [38].

[Fe-S] clusters are targets for ROS [39, 40]. Both H₂O₂ and superoxide can oxidize solvent-exposed labile [4Fe-4S]²⁺ clusters such as those of dehydratases, leading to the formation of [3Fe-4S]¹⁺ and the release of Fe, resulting in inactivation of enzymatic activity. In addition, H₂O₂ can attack nascent [Fe-S] clusters on carrier proteins during [Fe-S] cluster assembly [41]. Analysis of fprB and [Fe-S] cluster biogenesis in protection against oxidative stress revealed multiple and diverse roles of the enzyme in the process. First, the increased sensitivity of the mutant to the organic hydroperoxide CHP did not result from defects in [Fe-S] cluster biogenesis, because increased expression of isc-operon genes did not affect mutant sensitivity (Fig 6). Similarly, the sensitivities to diamide could not be complemented by pISC. This result suggests that [Fe-S] cluster biogenesis defects are not responsible for the fprB mutant sensitivity phenotype, suggesting that additional mechanisms partly contribute to the phenotypes of the mutant, such as oxidation of protein thiols by diamide at active sites or sites of structural importance and subsequent loss of function. Increasing [Fe-S] cluster biogenesis did partly complement the sensitivity phenotype of the mutant in response to H₂O₂, NaOCl and NaNO₂, implying that a decreased [Fe-S] cluster pool contributes to sensitivity of the mutant to these oxidants. Factors that may contribute to non- or partial complementation of the fprB oxidant-sensitive phenotype by pISC could be because [Fe-S] cluster assembly requires genes such as grxD (monothiol glutaredoxin) and nfuA ([Fe-S] cluster carrier protein), which are located outside the isc operon [42, 43]. In addition to the [Fe-S] cluster-related mechanism responsible for the phenotype, ROS can react with mononuclear iron proteins, leading to inactivation via the Fenton reaction. Fpr allows repair of oxidative damage to [Fe-S] clusters [19]. [4Fe-4S] cluster-containing hydratase enzymes such as aconitase or 6-phosphogluconate dehydratase could be reactivated by reactions catalyzed by Fpr [9]. The recovery of oxidatively damaged aconitase activity was slower for the fprB mutant than that for the wild type in P. putida KT2440 [13]. Nonetheless, the mutant could carry out the reactivation at a detectable rate, indicating that there are other reactivation pathways present [13].

The [4Fe-4S] electron carrier is highly susceptible to oxidation by superoxide anions/redox cyclers, accounting for the high sensitivity of the fprB mutant to these compounds. The sensitivity phenotype could be fully suppressed by the increasing supply of the [Fe-S] clusters through increased expression of genes from the isc operon, supporting the possibility that the fprB inactivation leads to the decrease in the [4Fe-4S] cluster supply via a decrease in reduced ferredoxin, a possible product of FprB-catalyzed reaction.

The physiological role of fprB in osmotic stress

The resistance of the fprB mutant toward various stress producing substances was determined. P. putida fpr mutants show growth defects under osmotic stress conditions that are partially complemented by iron supplementation to the growth media, suggesting that iron depletion is responsible for the mutant phenotype [13]. Hence, the role of PAO1 fprB in osmotic stress protection was tested. The results of plate sensitivity assays to salt stresses showed that the fprB mutant was highly sensitive to NaCl (0.5 M) and KCl (0.5 M) (Fig 7). High salt treatments caused 10³-fold (NaCl) and 10³-fold (KCl) decreases in percent-survival rates of fprB mutants compared with the parent strain PAO1 (Fig 7). The osmotic stress-sensitive phenotype could be fully complemented by expression of functional fprB in the fprB/pFprB strain (Fig 7). However, supplementing the medium with ferric or ferrous salts in various concentrations (0.05–1 mM) did not complement the osmotic sensitivity of the mutant (Fig 7). The results suggest that in PAO1, salt stress does not lead to intracellular iron depletion. Additional experiments were performed to test whether increased [Fe-S] cluster biogenesis by increased expression of genes from isc operon on a plasmid (pISC) could complement the salt sensitivity of the fprB mutant. These results showed that fprB/pISC expression could fully restore the salt stress hypersensitivity in the fprB mutant to the levels attained in PAO1 (Fig 7).

Fig 7. Determination of resistance to high salt conditions.

Plate sensitivity assays were performed to determine the levels of resistance of P. aeruginosa PAO1 and fprB mutant harboring empty vector (pBBR), pFprB, or pISC strains under conditions of either high sodium (NaCl, 0.5 M) or high potassium (KCl, 0.5 M) salts with/without ferrous (FeSO₄, 50 μM) or ferric (FeCl₃, 50 μM) supplementation. The data shown are the means and SD of percent survival at 18 h incubation from three independent experiments. The asterisk indicates a statistically significant difference (P < 0.01) compared to those of the PAO1/pBBR strain.

The results support that fprB has an important role in PAO1 survival under osmotic stress, similar to the result obtained for P. putida [13]. Nonetheless, the mechanisms responsible for the phenotype in the closely related bacteria are different, as the osmotic sensitivity could be complemented by increasing the expression of genes from the isc operon, indicating that [4Fe-4S] deficiencies in the P. aeruginosa mutant are likely responsible for the phenotype. In the PAO1 fprB mutant, increased sensitivity to high salt stress could result from the decrease in [4Fe-4S] cluster biogenesis and reduction of cluster availability, perhaps by reducing the functionality of [4Fe-4S] cluster-containing proteins that modulate the intracellular Na⁺/K⁺ contents. The reduced functionality of [4Fe-4S] cluster-containing proteins such as RnfB and RnfC, which are known to be involved in the Na⁺-translocation, are likely responsible for the phenotype of P. aeruginosa fprB mutant [44, 45].

fprB is required for protection against metal toxicity

P. aeruginosa has the ability to grow in diverse environmental niches. The physiological role of fprB in the protection against metal toxicity was also examined. First, the ability of the fprB mutant and PAO1 to survive in iron repletion and depletion conditions was examined. Several bacterial Fpr proteins have additional ferric reductase activity, which is important for the iron assimilation process [4, 8]. Exposure to toxic levels of iron (FeCl₃, 5.5 mM) caused a 10⁴-fold drop in percent survival of the mutant compared to PAO1 (Fig 8). Unexpectedly, growth in iron depletion conditions (induced via inclusion of an intracellular iron chelator, 2,2’-dipyridyl [DIPY], 1.2 mM) also led to a 10³-fold drop in the survival rate of the mutant (Fig 8). The ability to survive toxic concentrations of metals was further tested using different metal treatments in PAO1. Treatment of the fprB mutant with copper (CuCl₂, 4.2 mM), cobalt (CoCl₂, 0.5 mM), cadmium (CdCl₂, 0.8 mM), and zinc (ZnCl₂, 5 mM) caused 10³- to10⁴-fold reduction in survival percentages compared to the wild type. Treatment of the mutant with nickel (NiCl₂, 2.5 mM) and magnesium (MgCl₂, 15 mM), however, did not alter the percent survival compared to wild type. The increased sensitivity of fprB mutants to various metals could be fully complemented in the fprB/pFprB strain (Fig 8). Clearly, FprB has an important role in protecting cells from metal toxicity, though the question remained whether fprB mutant metal sensitivity phenotypes arose from a common defect or a defect in the ability to protect cells against levels of an individual metal. Here, we have shown that both the oxidative and osmotic stress sensitivity of the fprB mutant could be partially or wholly alleviated by increased expression of genes from the isc operon on a plasmid vector (Figs 6 and 7). Experiments were performed to test whether the expression of genes from the isc operon could protect the mutant from metal toxicity. The results of metal treatment on the mutant harboring pISC compared with control strains could be used to group metal treatments into three groups. Expression of genes from the isc operon partially complemented iron starvation conditions (from DIPY treatment) to a level 50-fold higher survival than the mutant but still 50-fold lower than that of PAO1 (Fig 8). The fprB/pISC showed less than 10-fold lower percent survival than wild type with the second group of metal treatments (repletion of FeCl₃ and CuCl₂), even though the mutant itself was highly sensitive (10³- to 10⁴-fold) (Fig 8). The mutant sensitivity to the last group of metals, CoCl₂, CdCl₂ and ZnCl₂ treatments, was fully complemented to PAO1 levels in the fprB/pISC strain (Fig 8). Expression of pISC in the mutant had no effects on the NiCl₂ and MgCl₂ treatments, similar to the fprB mutant response to these treatments (Fig 8).

Fig 8. Determination of resistance levels to metals, iron depletion and iron repletion conditions.

Plate sensitivity assays were performed to determine the resistance levels of P. aeruginosa PAO1 and fprB mutant harboring empty vector (pBBR), pFprB, or pISC strains against iron-chelating agent 2,2’-dipyridyl (DIPY, 1.2 mM), ferric iron (FeCl₃, 5.5 mM), copper (CuCl₂, 4.2 mM), cobalt (CoCl₂, 0.5 mM), cadmium (CdCl₂, 0.8 mM), zinc (ZnCl₂, 5 mM), nickel (NiCl₂, 2.5 mM), and magnesium (MgCl₂, 15 mM). The data shown are the means and SD of percent survival at 18 h incubation from three independent experiments. The asterisk indicates a statistically significant difference (P < 0.01) between the two indicated strains.

The increased sensitivity of the mutant to high FeCl₃ treatment and partial complementation by pISC suggests that in the fprB mutant, the decreased levels of reduced ferredoxin and the consequent decreased pool of [4Fe-4S] cluster increases iron availability and an insufficient transfer of this excess iron into storage. Therefore, accumulation of labile iron by the addition of excess iron led to cellular toxicity. Bacteria maintain a small pool of labile iron that is strictly controlled to assure sufficient concentration for growth while preventing its toxic accumulation [39, 46]. The [Fe-S] clusters could have an additional role as an iron sink to prevent excess labile iron from creating harmful side effects via the Fenton reaction. This rationale is supported by the observation that the expression of genes from pISC alleviates the sensitivity of the mutant to FeCl₃ treatment. Expression of genes from pISC increases [Fe-S] cluster assembly, thereby increasing iron sinks that can decrease toxic levels of labile iron pools. Iron depletion is a stressful condition for most organisms due to the requirement of iron in iron-containing cofactors such as heme and [Fe-S] clusters for the activity of many enzymes and proteins [12, 47]. The increased sensitivity of the mutant to iron depletion condition (via DIPY treatment) and partial complementation by isc operon expression suggests that low intracellular iron concentration causes reduced [Fe-S] biogenesis and subsequent reduction in functional [Fe-S] cluster-containing proteins. This deficiency could be partially compensated by increasing [Fe-S] biogenesis, although, as expected, increased [Fe-S] biogenesis alone could not fully overcome iron-depleted conditions. In addition, Fpr has a role in iron mobilization from storage [25], which is crucial under iron-depleted conditions.

[Fe-S] clusters and [Fe-S] cluster-containing enzymes/proteins are targets of reactive metals. The metal-[Fe-S] interactions often cause [Fe-S] cluster damage and an associated loss of function in [Fe-S] cluster-containing enzymes/proteins [48]. Copper toxicity has been shown to arise from its reactivity towards labile or solvent-exposed [Fe-S] cluster-containing proteins such as dehydratases, leading to the loss of iron atoms and subsequent loss of enzyme function [49]. Cobalt indirectly inactivates [Fe-S] clusters by reacting with damaged or newly synthesized clusters and forming mixed iron-cobalt-sulfur complexes that cause the loss of protein functions [50]. [Fe-S] cluster-containing enzymes are also targets of cadmium and zinc, and the ability of these metals to react with and damage [Fe-S] clusters correlate with their ability to bind sulfur [51]. The toxicities of these metals were shown to be more severe in the fprB mutant that had a [4Fe-4S] cluster biogenesis defect or redox imbalance. Furthermore, the ability of pISC to fully complement the increased metal sensitivity phenotype indicates that decreasing [4Fe-4S] cluster availability was responsible for the mutant increase in metal sensitivity. Treatments of the mutant with either nickel or magnesium ions that are nonreactive to [Fe-S] clusters did not alter the mutant sensitivity levels. This result is consistent with the role of deficient [Fe-S] cluster biogenesis in increasing the sensitivity of the mutant to reactive metals.

Conclusion

In sum, the regulation and patterns of stress-induced fprB expression suggests a correlation between levels of FprB, [4Fe-4S] clusters, and the ability of bacteria to respond to stress. IscR, a global regulator of the [Fe-S] biogenesis, is required for fprB expression during these conditions. IscR acts as a transcription activator of fprB expression via direct binding to a motif located near the fprB gene promoter. Furthermore, IscR provides an important link between cellular [Fe-S] cluster balance and fprB expression. Inactivation of fprB leads to a reduction in the availability of reduced ferredoxin, which is required for [4Fe-4S] cluster biosynthesis. Phenotypic analysis of the P. aeruginosa fprB mutant shows increased susceptibility to oxidative, osmotic and metal stress. A common theme among these diverse sources of stress is the ability to induce [Fe-S] cluster damages, leading to either a decrease in the [Fe-S] cluster pool available for [Fe-S] cluster-containing proteins and/or a loss of [Fe-S] clusters from associated proteins and their subsequent inactivation. The inability to mount a proper physiological response to stressful conditions arose from the insufficient pool of [4Fe-4S] clusters for [Fe-S] cluster-containing proteins in the fprB mutant, resulting in subsequent malfunction of these proteins and a defective in stress responses. This notion was supported by observations that increasing biogenesis of [Fe-S] clusters by high expression of the isc operon alleviated many of the physiological defects of the fprB mutant. Overall, the phenotypic analysis highlighted the important roles of [4Fe-4S] clusters in the bacterial stress response.

Methods

Bacterial strains, plasmids, and growth conditions

All bacterial strains and plasmids used in this study are listed in Table 1. Both E. coli and P. aeruginosa (PAO1) strains were aerobically cultivated in Luria-Bertani (LB) broth at 37°C with shaking at 180 rpm unless otherwise stated. An overnight culture was inoculated into fresh LB medium to give an optical density at 600 nm (OD_600nm) of 0.1. Exponential phase cells (OD_600nm of about 0.6, after 3 h of growth) were used in all experiments.

Table 1. Bacterial strains and plasmids used in this study.

Strain or Plasmid	Relevant characteristics	Source or Reference
P. aeruginosa
PAO1	Wild type	ATCC15692
fprB	fprB mutant, derivative of PAO1 in which fprB was disrupted by pKNOCKfprB, Gmr	This study
Fur	fur mutant	[58]
ΔiscR	iscR mutant, derivative of PAO1 in which a part of iscR was deleted	[32]
finR	finR mutant, derivative of PAO1 in which finR was disrupted by pKNOCKfinR, Gmr	This study
oxyR	oxyR mutant, derivative of PAO1 in which oxyR was disrupted by pKNOCKoxyR, Gmr	This study
soxR	soxR mutant, derivative of PAO1 in which soxR was disrupted by pKNOCKsoxR, Gmr	[33]
E. coli
DH5α	ϕ80d lacZΔM15, recA1, endA1, gyrA96, thi-1, hsdR17(rk −, mk +), supE44, relA1, deoR, Δ(lacYMA-argF)U169	Stratagene Inc. (USA)
BW20767	leu-63::IS10 recA1 creC510 hsdR17 endA1 zbf-5 uidA(ΔMlu1)::pir+ thi RP4-2-tet::Mu-1kan::Tn7	[59]
Plasmids
pKNOCKGm	Suicide vector, Gmr	[53]
pKNOCKfprB	pKNOCKGM containing a 247-bp fragment of fprB encoding region, Gmr	This study
pKNOCKfinR	pKNOCKGM containing a 284-bp fragment of finR encoding region, Gmr	This study
pKNOCKoxyR	pKNOCKGM containing a 291-bp fragment of oxyR encoding region, Gmr	This study
pBBR1-MCS4	Medium-copy-number expression vector, Apr	[55]
pFprB	pBBR1MCS-4 containing fprB, Apr	This study
pISC	pBBR1MCS-4 containing iscSUA-hscBA-fdx2-iscX coding regions, Apr	[32]
pIscR	pBBR1MCS-4 containing iscR, Apr	[32]
pUC18-miniTN7T::GM-lacZ	Transcriptional fusion vector with Tn7 insertion at a single site on the chromosome	[60]
pPfprB	pUC18-miniTN7T::GM-lacZ with fprB-promoter insertion at MCS	This study
pPfprBSD	pUC18-miniTN7T::GM-lacZ with site-directed mutagenic fprB-promoter insertion at MCS	This study

Gm^r, gentamicin resistance; Ap^r, ampicillin resistance

Molecular techniques

General molecular techniques including DNA and RNA preparations, DNA cloning, PCR amplification, Southern and Northern analyses and bacterial transformation were performed according to standard protocols [52]. The oligonucleotide primers used in this study are listed in Table 2.

Table 2. List of primers used in this study.

Primer	Sequence (5’→3’)	Purpose
BT87	CACTTAACGGCTGACATGG	Reverse primer in pKnockGm
BT543	TGACGCGTCCTCGGTAC	Forward primer in pKnockGm
BT2781	GCCCGCACAAGCGGTGGAG	Forward primer for 16S ribosomal gene
BT2782	ACGTCATCCCCACCTTCCT	Reverse primer for 16S ribosomal gene
BT3046	CCAGCGGGTCGGCATTCC	Forward primer for soxR expression
BT3047	AGGCCTGGAGCGACAGGC	Reverse primer for soxR expression
BT3334	TAGACGAGGAAGCCTGGATG	Forward primer for finR fragment
BT3335	TGTCCCTGGCCAACTGAG	Reverse primer for finR fragment
BT3351	ACCCGCCAGCCAGTTGTC	Forward primer for PA2274 expression
BT3352	CACGCTTTTCGCCCCCAG	Reverse primer for PA2274 expression
BT3458	AAGCCCAGCGGCAGCATC	Forward primer for fprB fragment
BT3459	GATCGAGACGAACGGCGC	Reverse primer for fprB fragment
BT3499	GTGCTTTGCGGGACACTAGG	Forward primer for full-length fprB
BT3500	GCTATCCGCCGCTACTGC	Reverse primer for full-length fprB
BT3551	GTCAACCGCAAGCGCTGATCG	Forward primer for fprB promoter analysis
BT3552	AGTCAGAGGCTGCACGTCGA	Reverse primer for fprB promoter analysis
BT3672	GAGCAGATCACCGGCTTC	Forward primer for anr expression
BT3673	GCAGTCTTCTTCGACAGCAG	Reverse primer for anr expression
BT4156	AGCAGGGCGAATTCGCCG	Forward primer for narG expression
BT4157	TCGTGGTTGGGCAGGTCC	Reverse primer for narG expression
EBI134	CAGCCGTACATCACCGAGAC	Forward primer for fprB promoter analysis
EBI157	GCGGGGATATTTACAAGCCTT	Forward primer for fprB promoter analysis with site-directed mutation
EBI158	AAGGCTTGTAAATATCCCCGC	Reverse primer for fprB promoter analysis with site-directed mutation
EBI163	TCGGCGCCATCTACACCATC	Forward primer for oxyR fragment
EBI164	GCAGGCTCTTGTCGTTGAG	Reverse primer for oxyR fragment
M13F	GTAAAACGACGGCCAGT	universal forward primer for expression vector
M13R	AAACAGCTATGACCATG	universal reverse primer for expression vector

Construction of P. aeruginosa fprB mutant

Insertional inactivation of fprB (PA4615) was performed using the pKNOCK suicide plasmid vector [53]. The internal DNA fragment of the fprB coding region was PCR-amplified with BT3458 and BT3459 primers, using PAO1 genomic DNA as template. The 247-bp PCR product was cloned into pKNOCK_Gm digested with SmaI, generating pKNOCK_Gm fprB. This recombinant plasmid was introduced into PAO1 by conjugation [54]. The trans-conjugants were selected by the Gm^r phenotype. A single homologous recombination event between the fprB fragment in the pKNOCK_Gm fprB and its counterpart on the chromosome causes insertional inactivation of fprB. The fprB mutant was confirmed by PCR and Southern blot analyses (S2 Fig).

Construction of P. aeruginosa finR and oxyR mutant

Insertional inactivation of the finR (PA3398) and oxyR was performed using pKNOCK vector [53]. The DNA fragments of the finR and oxyR coding regions were PCR- amplified from PAO1genomic DNA with BT3334 and BT3335 primers (for finR) and with EBI163 and EBI164 primers (for oxyR). The finR and oxyR mutants were constructed essentially as described for the fprB mutant.

Construction of pFprB

The full-length fprB was PCR-amplified from PAO1 genomic DNA with BT3499 and BT3500 primers. The 797-bp PCR product was cloned into the medium-copy-number expression vector pBBR1MCS-4 [55] cut with SmaI, yielding pFprB. The insert was sequenced to verify the correctness of the construct.

Northern blot analysis

RNA samples were prepared from 10 mL of an exponential phase cell cultures treated with/without oxidant for 15 min as previously described [54]. Total RNA isolation, agarose formaldehyde gel electrophoresis, blotting, and hybridization were performed as previously described [52]. A 247-bp fragment of the fprB coding region was amplified from pFprB using primers BT3458 and BT3459 and was used as a probe. The labeling of the DNA probe with [α-³²P]dCTP was performed using a DNA labeling bead (Amersham, GE Healthcare). The results from a representative experiment out of three independent experiments are shown. Densitometric analysis of the blot using ImageScanner III with LabScan 6.0 software (GE Healthcare) was performed to determine fold induction over the uninduced levels.

End-point RT-PCR

RNA samples were prepared from 10 mL of an exponential phase cell cultures treated with/without oxidant for 15 min as previously described [54]. Total RNA was extracted from oxidant-induced and uninduced cultures. RNA samples were treated with DNase I (Fermentas, Lithuania) according to the manufacturer's protocols. First-strand cDNA synthesis was performed using RevertAid M-MuLV Reverse Transcriptase with random hexamer primers (Fermentas, Lithuania). PCR was performed using 10 ng cDNA and a specific primer pair (BT3458 and BT3459 for fprB or BT2781 and BT2782 for the16S rRNA gene, which was used as an internal control) in a Taq PCR master mix kit (Fermentas, Lithuania). PCR amplification was carried out with an initial denaturation step at 95°C for 5 min, followed by 28 cycles of denaturation at 95°C for 15 s, annealing at 55°C for 15 s, and extension at 72°C for 15 s, and a final extension step at 72°C for 10 min. RT-PCR products were separated and visualized using agarose (1.8%) gel electrophoresis and ethidium bromide staining. Densitometric analysis of the blot using ImageScanner III with LabScan 6.0 software (GE Healthcare) was performed to determine fold induction over the uninduced levels.

Real-time RT-PCR

Cell culture conditions, RNA isolation, and reverse transcription was performed as described for end-point RT-PCR. Real-time RT-PCR was conducted using 10 ng cDNA as template, a specific primer pair and KAPA SYBR FAST qPCR kit. The reaction was run on Applied Biosystems StepOnePlus under the following conditions: denaturation at 95°C for 20 s, annealing at 60°C for 30 s, and extension at 60°C for 30 s, for 40 cycles. The specific primer pairs used for fprB, anr, narG, soxR, and PA2274 were BT3458-BT3459, BT3672-BT3673, BT4156-BT4157, BT3046-BT3047, and BT3351-BT3352, respectively. The primer pair for the 16S rRNA gene, which was used as the normalizing gene, was BT2781 and BT2782. Relative expression analysis was calculated using StepOne software v2.1 and is expressed as expression-fold change relative to the level of PAO1 wild type grown under uninduced condition. Experiments were repeated independently three times, and the data shown are means and standard deviations (SD).

Gel mobility shift assay

6×His-tagged IscR from PAO1 was purified as described [33]. Gel mobility shift assays were performed using a labeled probe containing either native or mutagenic fprB-promoters amplified from either pP_fprB or pP_fprB-SD, respectively, as a template and ³²P-labeled BT3551 and BT3552 primers. Binding reactions were conducted using 3 fmol of labeled probe in 25 μl of reaction buffer containing 20 mM Tris-HCl (pH 8.0), 50 mM KCl, 4 mM MgCl₂, 0.5 mM EDTA, 0.02 mg ml⁻¹ bovine serum albumin (BSA), 5 mM dithiothreitol (DTT), 10% (vol/vol) glycerol, and 200 ng of poly(dI-dC). Various amounts of purified IscR were added, and the reaction mixture was incubated at 25°C for 20 min. Protein-DNA complexes were separated by electrophoresis on a 7% non-denaturing polyacrylamide gel in 0.5x Tris-borate-EDTA buffer at 4°C and were visualized by exposure to X-ray film.

Enzymatic assays

Crude cell lysates were prepared from 10 mL of an exponential phase cell cultures treated with/without oxidant for 30 min as previously described [54]. Total protein concentration was determined using dye binding method (BioRad, USA). Succinate dehydrogenase activity assay was performed using method previously described [56] and enzyme activity was expressed as ΔA₆₀₀ per min per milligram protein. Aconitase activity assay was carried out using Aconitase Assay Kit (Abcam, UK). One unit of aconitase was defined as the amount of enzyme that isomerizes 1.0 μmol of citrate to isocitrate per min at pH 7.4 at 25°C.

Plate sensitivity assay

A plate sensitivity assay was performed to determine the oxidant resistance level as previously described [54]. Briefly, exponential phase cells were adjusted to OD₆₀₀ of 0.1 before making 10-fold serial dilutions. Then, 10 μl of each dilution was spotted onto LB agar plate containing appropriate concentrations of testing reagents. The plates were incubated overnight (about 18 h) at 37°C before the colony forming units (CFU) were scored. Percent survival was defined as the CFU on plates containing oxidant divided by the CFU on plates without oxidant and multiply by 100.

Bacterial killing assay

Killing assay was performed to determine the oxidant killing levels as previously described [54]. Briefly, the exponential phase cultures were adjusted to give an OD₆₀₀ of 0.5 before being treated with appropriate concentrations of oxidants for 30 min and were serially 10-fold diluted. 10 μL of diluted cultures was spot on the LB agar plate and incubated overnight (18 h). Cells survived killing treatments were scored by viable cell count. Percent survival was defined as the number of cells survived treatments divided by the number of cells in untreated control and multiply by 100.

Supporting Information

S1 Fig. Amino acid sequence alignment of Fpr in P. aeruginosa PAO1.

Alignment of P. aeruginosa FprA and FprB was performed using the CLUSTALW program. Black and light grey boxes indicate the subclass signature amino acid (F for subclass I Fpr and YW for subclass II Fpr) and the FAD-binding domain, respectively. The asterisk, colon, and period symbols indicate identical residues, conserved substitutions, and semi-conserved substitutions, respectively. Number indicates percent identity of the aligned protein with that of FprA.

(TIF)

S2 Fig. Southern blot analysis of the fprB mutation on P. aeruginosa genomes in a wild-type PAO1 and a fprB mutant.

Genomic DNA was extracted and digested with restriction enzyme, BclI. Digested DNA was run on 1% agarose gel and transferred into membrane. The membrane was hybridized with radioactive-labelled DNA fragment in the region of fprB gene. PAO1 gave a hybridized band of 1560 bp, while the fprB mutant gave a 3500-bp band. The radioactive-labelled lambda DNA EcoRI + HindIII were also presented in the reaction.

(TIF)

Data Availability

All relevant data are within the paper and its Supporting Information files.

Funding Statement

This work was supported by grants from the Center of Excellence on Environmental Health and Toxicology, Ministry of Education, Thailand (http://www.etm.sc.mahidol.ac.th/index.asp), the Chulabhorn Research Institute (http://www.cri.or.th/en/index.php) and by the Royal Golden Jubilee Ph.D. Program (PHD/0294/2550) from the joint funding of Thailand Research Fund and Mahidol University (http://rgj.trf.or.th/eng/rgje11.asp). Parts of this work are from A.R. dissertation submitted for a Ph.D. degree from Mahidol University. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.