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  • Research article
  • Open Access

Shewanella oneidensisHfq promotes exponential phase growth, stationary phase culture density, and cell survival

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BMC Microbiology201313:33

https://doi.org/10.1186/1471-2180-13-33

©  Brennan et al.; licensee BioMed Central Ltd. 2013

  • Received: 9 November 2012
  • Accepted: 21 January 2013
  • Published:

Abstract

Background

Hfq is an RNA chaperone protein that has been broadly implicated in sRNA function in bacteria. Here we describe the construction and characterization of a null allele of the gene that encodes the RNA chaperone Hfq in Shewanella oneidensis strain MR-1, a dissimilatory metal reducing bacterium.

Results

Loss of hfq in S. oneidensis results in a variety of mutant phenotypes, all of which are fully complemented by addition of a plasmid-borne copy of the wild type hfq gene. Aerobic cultures of the hfq∆ mutant grow more slowly through exponential phase than wild type cultures, and hfq∆ cultures reach a terminal cell density in stationary phase that is ~2/3 of that observed in wild type cultures. We have observed a similar growth phenotype when the hfq∆ mutant is cultured under anaerobic conditions with fumarate as the terminal electron acceptor, and we have found that the hfq∆ mutant is defective in Cr(VI) reduction. Finally, the hfq∆ mutant exhibits a striking loss of colony forming units in extended stationary phase and is highly sensitive to oxidative stress induced by H2O2 or methyl viologen (paraquat).

Conclusions

The hfq mutant in S. oneidensis exhibits pleiotropic phenotypes, including a defect in metal reduction. Our results also suggest that hfq mutant phenotypes in S. oneidensis may be at least partially due to increased sensitivity to oxidative stress.

Keywords

  • Shewanella oneidensis
  • Hfq
  • Metal reduction
  • Oxidative stress
  • Stationary phase survival

Background

Hfq is an RNA chaperone broadly implicated in sRNA function in many bacteria. Hfq interacts with and stabilizes many sRNAs, and it is thought to help promote sRNA-mRNA target interactions [1, 2]. Hfq protein monomers form a homohexameric ring that is thought to be the most active form of the protein [3, 4]. Much of what is known about Hfq function is drawn from studies of loss of function alleles of hfq in bacteria including Escherichia coli [5], Salmonella typhimurium [6], and Vibrio cholerae [7]. A common hfq mutant phenotype is slow growth through exponential phase. However, loss of hfq function usually results in an array of mutant phenotypes, many of which are bacterium-specific. For example, E. coli hfq mutants exhibit slow growth in vitro [5], survive poorly in stationary phase, and are sensitive to both H2O2 and hyperosmotic conditions [8]. In contrast, hfq mutants in Vibrio cholerae grow reasonably well in vitro (though they exhibit impaired growth in a mouse infection model), survive normally in stationary phase, and are fully resistant to both H2O2 and hyperosmotic conditions [7]. Since many of the sRNAs that have been characterized require Hfq for their function, perhaps it is not surprising that loss of Hfq compromises a wide array of cellular processes. However, the fact that hfq mutations in different bacteria produce distinct phenotypes suggests distinct evolutionary roles for both Hfq and sRNAs in these divergent bacteria.

Shewanella oneidensis is a Gram-negative γ-Proteobacterium that is a facultative anaerobe found in a wide range of environments. S. oneidensis is a member of a class of bacteria known as the dissimilatory metal-reducing bacteria (DMRB). Under anaerobic conditions, S. oneidensis has the ability to utilize an impressively wide range of both organic and metallic terminal electron acceptors. These metallic terminal electron acceptors include Cr(VI), Fe(III), Mn(III) and (IV), and U(VI) [9, 10]. The ability to mitigate the toxicity of soluble Cr(VI) and U(VI) by reduction to insoluble oxides of Cr(III) and U(IV), respectively, makes Shewanella an attractive potential bioremediating organism. In addition, the ability to deliver electrons to the extracellular environment allows Shewanella to generate electrical current in microbial fuel cells [11]. Because the transition between aerobic and anaerobic metabolism is likely to occur frequently in nature, it is probable that sRNAs play a role in the transition between these metabolic states in S. oneidensis.

To gain insight into the functions of Hfq in S. oneidensis, we have constructed and characterized a null allele of the hfq gene. The hfq∆ mutation in S. oneidensis is pleiotropic, resulting in defects in aerobic growth and greatly reduced recovery of colony forming units (CFU) from stationary phase cultures. In addition, loss of hfq results in compromised anaerobic growth on fumarate and diminished capacity to reduce Cr(VI). Finally, we have found that the S. oneidensis hfq∆ mutant is highly sensitive to oxidative stress. Importantly, each of the hfq mutant phenotypes we have described is complemented by a plasmid-borne copy of the wild type S. oneidensis hfq gene, strongly suggesting that the mutant phenotypes we have observed are the result of the loss of hfq and not due to disruption of another gene. Our results suggest that Hfq in S. oneidensis is involved in both common and organism-specific regulatory processes. To our knowledge, this is the first characterization of an hfq mutant in a dissimilatory metal reducing bacterium.

Methods

Media and growth conditions

Aerobic cultures were grown in either LB (10g/L tryptone, 5g/L yeast extract, 10g/L NaCl) or a modified version of the original M1 medium [9] with 30mM lactate as the electron donor. The modified M1 medium used in this study contains buffer/salts (3mM PIPES buffer, pH 7.0, 28mM NH4Cl, 1.34mM KCl, 4.4mM NaH2PO4, 125mM NaCl), vitamins [81.8nM D-biotin (vitamin B7), 45.3nM folic acid (vitamin B9), 486.4nM pyridoxine HCl (vitamin B6), 132.8nM riboflavin (vitamin B2), 133.6nM thiamine HCl (vitamin B1), 406.2nM nicotinic acid (vitamin B3), 209.8nM D-pantothenic acid, 0.74nM vitamin B12, 364.6nM p-aminobenzoic acid, 242.4nM lipoic acid], minerals [78.5μM nitriloacetic acid (trisodium salt), 249.1μM MgSO4 · 7 H2O, 29.6μM MnSO4 · 1 H2O, 171.1μM NaCl, 3.6μM FeSO4 · 7 H2O, 6.8μM CaCl2 · 2 H2O, 4.2μM CoCl2 · 6 H2O, 9.54μM ZnCl2, 0.4μM CuSO4 · 5 H2O, 0.21μM AlK(SO4)2 · 12 H2O, 1.61μM H3BO3, 1.24μM Na2MoO4 · 2 H2O, 1.01μM NiCl2 · 6 H2O, 0.76μM Na2WO4 · 2 H2O], and amino acids (135.9μM L-glutamic acid, 114.8μM L-arginine, 190.3μM DL-serine). Anaerobic cultures were grown in modified M1 medium with 30mM lactate as the electron donor and 30mM sodium fumarate as the electron acceptor. Anaerobic conditions in broth cultures were achieved by treating cultures in sealed test tubes using Oxyrase for Broth (Oxyrase, Inc., Mansfield, Ohio) as per the manufacturer’s instructions.

All S. oneidensis cultures were grown at 30°C, while E. coli cultures were grown at 37°C. Cultures containing both E. coli and S. oneidensis were grown at 30°C. Antibiotics were used at the following concentrations: Gentamicin (Gm): 5 μg/ml; Tetracycline (Tc): 10 μg/ml for E. coli; 1 μg/ml for S. oneidensis, [we used a lower concentration of Tc for selection of S. oneidensis than for E. coli because we found that the minimum inhibitory concentration (MIC) of Tc for S. oneidensis MR-1 is <1 μg/ml (data not shown)]; Kanamycin (Km): 25 μg/ml; Ampicillin (Amp): 100 μg/ml.

For growth curves, 5ml LB Km cultures of S. oneidensis strains were inoculated from frozen permanent stocks and aerobically outgrown overnight (10–12 hours). The overnight cultures were diluted in LB Km to an ABS600 ≅ 0.1 or in modified M1 Km to an ABS600 ≅ 0.025 and aerobically outgrown to log phase (ABS600 ≅ 0.4-0.8). These exponentially growing cultures were then diluted to an ABS600 ≅ 0.1 (LB Km) or to an ABS600 ≅ 0.025 (modified M1 Km). Aerobic cultures (15-20ml) were grown in 125mL Erlenmeyer flasks shaken at 250RPM. Anaerobic cultures (15ml) were grown in sealed test tubes without shaking. Culture densities (ABS600) were monitored spectrophotometrically, and culture titers (CFU/ml) were determined by plating serial dilutions of cultures on LB Km plates.

Construction of the S. oneidensis hfq∆ mutant and hfqrescue construct

To generate a null allele of hfq (So_0603 [12]) we deleted most of the hfq open reading frame and replaced it with a promoterless lacZ/gentamicin resistance gene cassette from pAB2001 [13]. We first PCR amplified a 5′ fragment using the primers GGCCCCGGGTAGAGCAAGGCTTTATTGATGAGGTAGC and GGCGCATGCGTCTTGTAAAGATTGCCCCTTAGCC and a 3’ fragment using the primers GGCGCATGCACGATATGCCAAGTGGCGAATAAGG and GGCGGTACCAGCTCGTTGGGCGAAAATATCCAAAATCAG. Following restriction (restriction endonucleases purchased from New England Biolabs, Ipswich, MA) of the 5′ PCR fragment with XmaI and SphI and restriction of the 3’ PCR fragment with SphI and KpnI, the two fragments were simultaneously ligated into pBSKS II + [14] that had been restricted with XmaI and KpnI. A 4.5kb SphI fragment from pAB2001 was then inserted into the SphI site of this plasmid to generate pBS-hfq∆. The XmaI-KpnI fragment from pBS-hfq∆, which contained the lacZ/gentamicin-disrupted hfq gene, was then cloned into XmaI/KpnI restricted pDMS197 [15], a R6K ori plasmid. The resulting plasmid, pDMS197-hfq∆ was transformed into E. coli SM10λpir [16], mated into S. oneidensis MR-1 [9], and Gmr/Tcr single crossover recombinants were isolated. Following growth in LB liquid without selection, cultures of these single crossovers were plated to LB plates containing Gm, 5% sucrose (w/v), and 0.1% NaCl (instead of omiting NaCl to increase the likelihood of isolating an hfq mutant in the event that loss of hfq resulted in cells sensitive to hypoosmotic conditions). Gmr Sucr Tcshfq∆ mutant candidates were screened via PCR and DNA sequencing of the disrupted region. The sequence of the primers used for diagnostic PCR in Figure 1 are as follows: A (hfq 5’ diagnostic) - ATAATGTGGTGCAATTTGCC; B (lacZ 5’ out) - CGTTGTAAAACGACGGGATCG; C (aacC1 3’out) - GATGCACTTTGATATCGACCC; D (hfq 3’ diagnostic) - GAGTCCAACCACGCACTAGG.
Figure 1
Figure 1

Construction and verification of a null allele of the Shewanella oneidensis MR-1 hfq gene. (A) Knockout strategy for the MR-1 hfq gene. Most of the hfq gene coding sequence (all but the first 9 codons and last 6 codons) was replaced with a cassette containing a promoterless lacZ gene and a gentamicin resistance marker. (B) Agarose gel of analytical PCR reactions using wild type MR-1 (lanes 2–4) or hfq∆ mutant (lanes 5–7) templates and primers A, B, C, and D (see Materials and Methods for primer sequences) indicated with arrows on the diagram in panel (A) The size standard (M) in lane 1 is 1kb plus DNA ladder (Invitrogen). (C) Western blot of SDS-PAGE-fractionated total protein from various Shewanella strains probed with a polyclonal antibody raised against E. coli Hfq protein. Lanes 1 and 2: MR-1 containing pBBR1-MCS-2 (vector) or hfq rescue construct (phfq), respectively. Lanes 3 and 4: hfq∆ containing vector or phfq, respectively. The antibody detects both putative Hfq monomers (~10kDa) as well as putative Hfq homohexamers (~60kDa).

To generate an hfq rescue construct, we PCR amplified a 1.3kb genomic fragment containing the S. oneidensis MR-1 hfq coding sequence and ~1kb upstream of the hfq open reading frame. Based on hfq promoter analysis in E. coli, this fragment likely contains the native promoters for S. oneidensis hfq [17]. A PCR product was generated using the 5’ primer GGCAAGCTTCAGGAAAAACGGCTTTAGCTCTCG and the 3’ primer GGCGGTACCACTAAACCTTATTCGCCACTTGGC. Following restriction with HindIII and KpnI, this PCR product was ligated to HindIII/KpnI restricted pBBR-1MCS2 [18]. The resulting plasmid, pBBR1-hfq, was transformed into E. coli S17-1λpir [19] and mated into S. oneidensis strains. In our hands, the pBBR1-MCS2 based vectors were stably maintained in S. oneidensis strains after 30 hours in LB Km cultures and after 120 hours in modified M1 Km cultures (data not shown).

Western blot analyses

3ml aliquots of S. oneidensis cultures were pelleted in a microcentrifuge for 2’ at 20300 x g. Bacterial pellets were frozen at −80°C, thawed, and then treated with Bacterial Protein Extraction Reagent (B-PER) in the presence of 100μg/ml lysozyme, 5U/ml DNAse I, and 1X Halt Protease Inhibitor Cocktail. Protein was quantified using the Pierce BCA Protein Assay Kit as per manufacturers instructions (all reagents were obtained from Thermo Scientific, Rockford, IL).

For western blot analysis, 90μg of protein per lane was size fractionated at 4°C using Any kD Mini-PROTEAN TGX Precast Gels (Bio-Rad, Hercules, CA). Proteins were then transferred to an Immobilon-PSQ PVDF membrane (EMD Millipore, Billerica, MA). Equivalent protein in different lanes was verified by Ponceau S staining of the membrane (data not shown). The membrane was blocked for 1 hour at room temperature using LI-COR Odyssey Blocking Buffer (LI-COR Biosciences, Lincoln, NE) and probed with a 1:5000 dilution of primary antibody, rabbit anti-E. coli Hfq [20] overnight at 4°C. The blot was washed 4 times for 5 minutes each with PBS-T and then probed with a 1:10000 dilution of goat anti-rabbit secondary antibody conjugated to IRDye 800CW Infrared Dye (LI-COR Biosciences, Lincoln, NE) for 45 minutes at room temperature (~22°C). The blot was washed with PBS-T 4 times for 5 minutes each and then rinsed with PBS to remove residual Tween 20. The blot was then imaged on a LI-COR Odyssey infrared scanner. Protein in Figure 1C was harvested from 24 hour old LB Km cultures. Older cultures consistently accumulated higher levels of Hfq protein, though our western blot results were consistent regardless of culture age at harvest; we never observed Hfq protein in the hfq∆/empty vector cultures (Figure 1C and data not shown).

Chromium reduction assays

Chromium reduction assays were performed using a diphenylcarbazide-based quantitative, valence state specific, colorimetric assay for Cr(VI) [21]. Log phase cultures (ABS600 ≅ 0.5-0.8) grown in modified M1 medium were diluted to ABS600 ≅ 0.4 in modified M1 medium that had been prewarmed to 30°C. The cultures were transferred to sealed test tubes and treated for 30 minutes at 30°C with Oxyrase for Broth (Oxyrase, Inc., Mansfield, Ohio) to remove oxygen. Following addition of 100μM K2CrO4, cultures were incubated without shaking in a 30°C water bath in sealed test tubes. 1ml aliquots of cultures were periodically removed and added to 13mm borosilicate glass tubes containing 0.25ml of a 0.5% diphenylcarbazide solution in acetone and 2.5ml 0.28N HCl. Following vortexing, ABS541 values for individual samples were measured in a SPECTRONIC 20D+ spectrophotometer (Thermo Scientific, Rockford, IL).

Oxidative stress assays

Overnight cultures grown in LB Km were diluted to an ABS600 ≅ 0.1. These cultures were outgrown for 2–3 hours to exponential phase (ABS600 ≅ 0.4-0.6) then diluted to an ABS600 ≅ 0.2. Following five minutes of aerobic growth, cultures were treated with H2O (mock), 0.4 mM H2O2 to induce peroxide stress, or 5 mM methyl-viologen (paraquat) to induce superoxide stress. Cultures were then grown aerobically for 15 minutes. Following treatment, each culture was serially diluted in triplicate in phosphate-buffered saline (PBS, pH 7.4). The dilutions were plated to LB Km plates within five minutes of harvest and grown overnight before scoring.

Results

Construction and verification of a null allele of hfq in Shewanella oneidensisMR-1

To study the roles played by the hfq gene in Shewanella oneidensis, we constructed a null allele of the putative hfq gene (So_0603) in S. oneidensis strain MR-1 [9, 12]. To disrupt the S. oneidensis hfq gene, we generated a knockout construct in which we replaced most of the coding region of hfq with a cassette derived from pAB2001 [13] containing a promoterless lacZ gene and a gentamicin resistance marker (Figure 1A - see Materials and Methods for details). This knockout fragment was cloned into the TcrsacB-counterselectable R6K ori suicide vector pDMS197 [15] and mobilized into S. oneidensis MR-1. Single crossovers of the hfq knockout plasmid into the MR-1 genome were isolated on the basis of both Gm resistance and ability to grow on modified M1 defined medium. Following PCR verification, LB cultures of Gmr Tcr single crossovers were outgrown in LB medium without antibiotic selection and then plated on LB agar containing Gm and 5% (w/v) sucrose. Elimination of the hfq gene in Sucr Tcs candidates was verified by PCR analyses (Figure 1B) and DNA sequencing analysis (data not shown). Western blotting demonstrated that the hfq∆ strain fails to produce Hfq protein (Figure 1C). Taken together, these data indicate that we have generated a null allele of hfq in S. oneidensis.

The Shewanella oneidensis hfqmutant is defective in aerobic growth and exhibits reduced viable cell counts in stationary phase

Because mutations in the hfq gene compromise growth in many bacteria, we analyzed the growth properties of the S. oneidensis hfq null mutant. We characterized four strains: MR-1 containing pBBR1-MCS2 (hereafter referred to as empty vector), MR-1 containing pBBR1-hfq (pBBR1-MCS2 containing the wild type hfq gene under the control of its putative native promoter, hereafter referred to as phfq), hfq∆ containing empty vector, and hfq∆ containing phfq. Loss of the hfq gene resulted in a small colony phenotype on both LB agar plates (Figure 2A) and modified M1 defined medium plates (data not shown). The small colony phenotype of the hfq mutant was completely rescued by phfq, but not by the empty vector alone (Figure 2A). The growth phenotype of wild type MR-1 cells containing the phfq rescue plasmid was indistinguishable from MR-1 cells containing the empty vector (Figure 2A), suggesting that additional, plasmid-borne copies of hfq that result in higher Hfq protein levels than found in wild type cells (Figure 1C) do not significantly affect the growth of S. oneidensis on solid media. Of note is that the hfq mutant colonies with empty vector never attain the same colony size as strains harboring wild type hfq, even after extended incubation (data not shown).
Figure 2
Figure 2

Shewanella oneidensis Hfq promotes exponential growth, terminal culture density, and viable cell counts in stationary phase. Growth of MR-1/empty vector, MR-1/phfq, hfq∆ /empty vector, and hfq∆ /phfq on LB agar containing kanamycin (A), in LB liquid containing kanamycin (B), or in modified M1 defined medium containing kanamycin (C). Plates in (A) were photographed after 24 hours of growth following inoculation from frozen permanent stocks. Three independent liquid cultures of each strain tracked in (B-D) were inoculated with log phase cultures grown in LB (B and D) or modified M1 medium (C). (D) Analysis of the relationship between viable cell counts (CFU/ml) and culture turbidity (ABS600) in LB cultures. Data points marked with “#” have CFU/ml/ABS600 values of zero. Error bars in panels (B-D) indicate a 99% confidence interval (P = 0.01).

To further characterize the nature of the growth defect in the hfq mutant, we compared the growth of the hfq mutant in aerobic liquid cultures to strains containing one or more wild type copies of the hfq gene (Figure 2B). When exponentially-growing cultures were diluted to late lag phase and outgrown beyond stationary phase, we consistently observed that the hfq∆/empty vector culture densities were significantly lower than those of the MR-1/empty vector cultures through exponential phase. In addition, the terminal cell densities of stationary phase hfq∆/empty vector cultures were significantly lower than the terminal cell densities of MR-1/empty vector cultures (Figure 2B). We also observed delayed growth during exponential phase and lower terminal stationary phase densities in hfq∆/empty vector liquid cultures grown in modified M1, a defined medium (Figure 2C). The growth and terminal density defects of the hfq mutant in liquid cultures were completely rescued by phfq, as the growth of the hfq∆/phfq strain was indistinguishable from that of MR-1/empty vector in both LB (Figure 2B) and modified M1 (Figure 2C). Finally, extra copies of hfq that result in higher Hfq protein levels (Figure 1C) do not appear to alter the growth of S. oneidensis in liquid medium, as growth of MR-1/phfq and hfq∆/phfq cultures was indistinguishable from that of MR-1/empty vector cultures in LB and modified M1 media (Figures 2B and 2C).

To determine whether the relationships between spectrophotometric measurements of culture density and cell number were comparable between the strains used in our study, we determined the relationship between ABS600 values and viable cell counts for MR-1/empty vector, MR-1/phfq, hfq∆/empty vector, and hfq∆/phfq at various times during culture outgrowth. In both LB cultures (Figure 2D) and modified M1 cultures (data not shown), the relationship between ABS600 and colony forming units per ml (CFU/ml) was consistent for all four strains throughout exponential phase and until approximately mid-stationary phase. This indicates that the optical properties of the four strains characterized are highly similar at 600nm and that turbidity measurements are an accurate indicator of culture growth until mid stationary phase.

Intriguingly, we observed that the CFU/ml/ABS600 values for the four strains used in our studies diverged dramatically following mid-stationary phase (Figure 2D). We consistently found that hfq∆/empty vector cultures experienced a precipitous drop in CFU counts late in stationary phase. In most cases, culturable cell counts had dropped to zero CFU/ml by 30 hours. In contrast, MR-1/empty vector cultures were much more robust than hfq∆ /empty vector cultures, maintaining significant CFU counts, even after 30 hours of growth. The data presented in Figure 2D represents a typical result for an iteration of this experiment. It is worth noting, however, that the timing of the beginning of the reduction in CFU counts observed for the MR-1/empty vector strain and for the hfq∆/empty vector strain could vary by several hours between independent cultures, even parallel cultures simultaneously inoculated using the same preculture (data not shown). Furthermore, we also consistently observed that MR-1/phfq and hfq∆/phfq cultures, which contain more Hfq protein than wild type cultures at 24 hours (Figure 1C), retained significantly higher numbers of colony forming units compared to MR-1/empty vector cultures in extended stationary phase. Taken together, our loss-of-function and gain-of-function analyses demonstrate that Hfq promotes cell survival or culturability in extended stationary phase.

The hfq∆mutant is impaired in anaerobic growth and chromium reduction

To characterize the role of S. oneidensis hfq in anaerobic growth, we compared the growth kinetics of strains MR-1/empty vector, MR-1/phfq, hfq∆/empty vector, and hfq∆ /phfq grown in modified M1 defined medium with fumarate as the terminal electron acceptor. Similar to the growth defects observed during aerobic growth, anaerobic hfq∆ /empty vector cultures grew more slowly during exponential phase and reached a lower terminal density than MR-1/empty vector cultures. (Figure 3A). The growth and terminal density defects of hfq mutant cultures in anaerobic modified M1 plus fumarate were completely rescued by phfq, as the growth of the hfq∆/phfq strain was indistinguishable from that of MR-1/empty vector (Figure 3A). Extra copies of hfq did not alter the ability of S. oneidensis to utilize fumarate as a terminal electron acceptor, as growth of MR-1/phfq and hfq∆/phfq cultures was very similar to that of MR-1/empty vector cultures (Figure 3A).
Figure 3
Figure 3

The hfq∆ mutant is deficient in anaerobic respiration. (A) Growth of MR-1/empty vector, MR-1/phfq, hfq∆ /empty vector, and hfq∆ /phfq under anaerobic conditions with fumarate as the terminal electron acceptor. Data presented is from three independent cultures. Error bars represent a 99% confidence interval (P = 0.01). (B and C) Results of chromium reduction assays. Chromium reduction/disappearance of Cr(VI) was assayed using the diphenylcarbazide method. Error bars represent a 99% confidence interval (P = 0.01). (D) Quantification of the rate of Cr(VI) reduction (expressed as the change in ABS541 per minute per ABS600) in the cultures tracked in (C) above during the first five minutes following the addition of chromium to anaerobic cultures. Error bars represent the standard deviation for triplicate cultures. ** indicates that the hfq∆ /empty vector rate is statistically different from the other three strains (P < 0.002 for all three comparison in unpaired two-tailed Student’s T-tests).

To determine whether loss of hfq altered the ability of S. oneidensis to utilize chromium as a terminal electron acceptor, we measured the kinetics of Cr(VI) reduction by our four hfq strains using diphenylcarbazide, a reagent that binds to Cr(VI) and produces a purple color proportional to the amount of Cr(VI) in the sample [21]. In fully anaerobic cultures with no other electron acceptor present, metal reduction begins immediately upon addition of Cr(VI), and the rate of reduction is highest in the first five minutes following Cr(VI) addition. As the Cr(VI) is reduced, the assay results proceed from a deep purple color at early timepoints to a colorless solution at later timepoints, allowing quantification of the disappearance of Cr(VI) (Figure 3B). In our assays, the ABS541 values for the assay timepoints do not fall below ~0.2 because of the absorbance contribution of the cells at 541nm (data not shown). Though all strains tested eventually reduced all of the detectable Cr(VI), we found that the hfq∆ mutant is significantly slower in reducing Cr(VI) and takes nearly twice as long to utilize all available Cr(VI) as strains containing wild type hfq (Figures 3B and 3C). In addition, the rate of Cr(VI) reduction (∆ABS541) per minute per ABS600 unit during the first five minutes of metal reduction for the hfq∆/empty vector strain was less than half that of strains containing at least one copy of wild type hfq (Figure 3D).

To be certain that the Cr(VI) reduction defect observed in the hfq∆/empty vector strain was due to a defect in metal reduction and not death of cells due to an increased sensitivity to Cr, we measured the CFU/ml present in cultures of all four strains both before and after the 30 minute chromium reduction assay. We found no significant differences in the CFU/ml values measured before and after the assay for any of the four strains used in our experiments (data not shown). As observed in our growth analyses above, the CFU/ml/ABS600 values for the four anaerobic strains did not vary significantly among the cultures (data not shown), demonstrating again that turbidity measurements were an accurate reflection of viable cell counts. Taken together, our results suggest that hfq∆/empty vector cells have an intrinsic defect in use of chromium as a terminal electron acceptor during anaerobic respiration.

The hfq∆mutant is highly sensitive to oxidative stress

Mutations in hfq in E. coli result in an increased sensitivity to oxidative stress in addition to poor survival in stationary phase [8]. Given the poor survival of the S. oneidensis hfq∆ mutant in extended stationary phase, a period typically characterized by increased oxidative stress [22, 23], we decided to explore the ability of the hfq∆ mutant to cope with oxidative stress. Exponentially growing cultures of MR-1/empty vector, MR-1/phfq, hfq∆/empty vector, and hfq∆/phfq were treated with either H2O2 to induce peroxide stress or methyl viologen to induce superoxide stress. Serial dilutions of these cultures were then plated, and the survival rates relative to mock (H2O) treated cultures were measured. The survivorship of each strain was determined by calculating the ratio of viable cells in the treated cultures to viable cells in the mock treated cultures. Strains with a wild type copy of hfq survived significantly better than the hfq∆/empty vector strain when challenged with either H2O2 (Figure 4A and 4B) or methyl viologen (Figure 4C and 4D). These data suggest that one function of S. oneidensis Hfq is to protect cells against oxidative stress.
Figure 4
Figure 4

The hfq∆ mutant is highly sensitive to oxidative stress. Aerobic, exponentially growing cultures of MR-1/empty vector, MR-1/phfq, hfq∆ /empty vector, and hfq∆ /phfq were treated for 15 minutes with either (A and B) 0.4 mM H2O2 or (C and D) 5mM methyl viologen (paraquat) and then immediately titered. Survivorship ratios were determined by calculating the ratio of the number of viable cells in the treated cultures to the number of viable cells in mock (H2O) treated cultures. Values on the graphs are the mean survivorship ratios for three independent experiments. Error bars in (A) and (C) indicate standard deviations. The hfq∆ /empty vector survival rate is statistically different from the other three strains in both the H2O2 and methyl viologen experiments (** indicates that P < 0.005 for comparison of the hfq∆ /empty vector strain data to each of the other strains in unpaired two-tailed Student’s T-tests). Panels (B) and (D) demonstrate typical ten-fold dilution series results obtained after treatment of strains MR-1/empty vector, MR-1/phfq, hfq∆ /empty vector, and hfq∆ /phfq with (B) H2O (mock) or H2O2 or (D) H2O (mock) or methyl viologen.

Discussion and conclusions

In this paper, we describe the construction and characterization of a null allele of the hfq gene in the bacterium S. oneidensis. Loss of the hfq gene produces an assortment of phenotypes, each of which is fully complemented by an exogenously supplied copy of the wild type hfq gene. To our knowledge, this is the first report of an hfq gene knockout in a dissimilatory metal reducing bacterium. Given the varied roles played by Hfq in diverse bacteria, we expect that this mutant will be both a useful tool for analyzing sRNA function in S. oneidensis as well as for understanding Hfq function in general.

It is clear from our analyses that S. oneidensis Hfq positively regulates exponential phase growth. The exponential phase growth defect of the hfq mutant is not growth medium specific, as we observe slow exponential phase growth in both complex and defined media. In addition, we observe this defect when cells are grown under both aerobic and anaerobic conditions. It is not yet clear why the hfq mutant grows slowly when nutrients are plentiful. It is possible that the hfq mutant growth phenotype is a result of a defect in nutrient acquisition, a possibility suggested by the fact that hfq mutants in a variety of bacteria express lower levels of genes involved in nutrient uptake [6, 24–26]. It is also possible that the hfq mutant has more general set of metabolic defects that underlie its slow growth phenotype, which may explain why the hfq mutant is less efficient in Cr(VI) reduction. Alternatively, hfq may have a more specific role in utilization of Cr(VI) as a terminal electron acceptor.

A second notable hfq mutant growth phenotype is the failure of mutant cultures to achieve a terminal cell density as high as those seen in wild type cultures. Though it is not yet clear what underlies this mutant phenotype, it is possible that the hfq mutant is unable to fully utilize the available nutrients in the medium or that it exhausts a nutrient that is rate limiting for growth more rapidly than wild type cells. Alternatively, the hfq mutant may produce more of, or be more sensitive to, at least one growth-suppressing product produced during S. oneidensis growth.

Strikingly, S. oneidensis hfq mutant cultures exhibit a severe loss of colony forming units in stationary phase, with cultures often displaying no detectable CFU. One possibility is that Hfq promotes cell survival in stationary phase, and thus loss of hfq results in loss of culture viability. An alternative explanation is that Hfq functions to prevent cells from entering a viable but not culturable (VBNC) state [27], and thus reduced CFU/ml counts in hfq∆ mutant cultures are due to hfq∆ cells precociously assuming VBNC status. Both of these models are supported by the fact that moderate overexpression of Hfq results in higher CFU/ml counts during stationary phase when compared to cells with wild type Hfq protein levels. Further experimentation will be required to differentiate between these two possible explanations for the greatly reduced CFU/ml counts in hfq∆ stationary phase cultures.

Because the hfq mutant is highly sensitive to oxidative stress, it is possible that the stationary phase survival defect in hfq mutant cells is a consequence of poor resistance to oxidative stress. Multiple Hfq-dependent sRNAs (arcZ, dsrA, and rprA) positively regulate expression of the stationary phase sigma factor RpoS in other systems [28–30]. Thus, it is possible that loss of Hfq in S. oneidensis causes low rpoS expression, resulting in poor induction of the rpoS regulon. Lower rpoS regulon induction may increase the oxidative stress sensitivity of the hfq mutant and consequently reduce stationary phase survival. Another possibility that remains to be explored is whether the hfq mutant’s sensitivity to oxidative stress is due to altered function of superoxide dismutase (sodB – So_2881) and/or one or more of the four genes predicted to encode proteins with catalase activity katB (So_1070), So_1771.2, katG2 (So_4405), and katG1 (So_0725)] [12]. Finally, it will be of interest to determine whether S. oneidensis contains an hfq-dependent OxyR-OxyS system that is involved in response to oxidative stress as in other systems [20, 31].

We are currently investigating the mechanisms by which S. oneidensis Hfq promotes growth, terminal culture density, and stationary phase survival. However, given that Hfq has been broadly implicated in the function of many sRNAs in other systems [32], the S. oneidensis hfq mutant generated in this study will facilitate analysis of the roles of Hfq and sRNAs in adaptation to a wide range of environmental conditions. This is of particular interest since a previous study demonstrated that S. oneidensis sRNAs do not always have completely overlapping functions with their homologs in other systems [33].

Declarations

Acknowledgements

We thank Aixia Zhang for supplying the anti-Hfq antibody. Thanks to Fr. Nicanor Austriaco, O.P. and Jennifer Gervais for thoughtful discussions and critical reading of the manuscript. Research reported in this publication was supported by an Institutional Development Award (IDeA) from the National Institute of General Medical Sciences of the National Institutes of Health under grant number 8 P20 GM103430-12. Additional funding was provided by a Providence College Undergraduate Research Grant to CMB and an American Society for Microbiology (ASM) Summer Research Fellowship to MTG.

Authors’ Affiliations

(1)
Department of Biology, Providence College, Providence, RI, USA

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© Brennan et al.; licensee BioMed Central Ltd. 2013

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