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The Alternative Role of Enterobactin as an Oxidative Stress Protector Allows Escherichia coli Colony Development

  • Conrado Adler ,

    Contributed equally to this work with: Conrado Adler, Natalia S. Corbalan

    Affiliation Departamento de Bioquímica de la Nutrición, INSIBIO (Consejo Nacional de Investigaciones Científicas y Técnicas-Universidad Nacional de Tucumán) San Miguel de Tucumán, Tucumán, Argentina

  • Natalia S. Corbalan ,

    Contributed equally to this work with: Conrado Adler, Natalia S. Corbalan

    Affiliation Departamento de Bioquímica de la Nutrición, INSIBIO (Consejo Nacional de Investigaciones Científicas y Técnicas-Universidad Nacional de Tucumán) San Miguel de Tucumán, Tucumán, Argentina

  • Daiana R. Peralta,

    Affiliation Departamento de Bioquímica de la Nutrición, INSIBIO (Consejo Nacional de Investigaciones Científicas y Técnicas-Universidad Nacional de Tucumán) San Miguel de Tucumán, Tucumán, Argentina

  • María Fernanda Pomares,

    Affiliation Departamento de Bioquímica de la Nutrición, INSIBIO (Consejo Nacional de Investigaciones Científicas y Técnicas-Universidad Nacional de Tucumán) San Miguel de Tucumán, Tucumán, Argentina

  • Ricardo E. de Cristóbal,

    Affiliation Departamento de Bioquímica de la Nutrición, INSIBIO (Consejo Nacional de Investigaciones Científicas y Técnicas-Universidad Nacional de Tucumán) San Miguel de Tucumán, Tucumán, Argentina

  • Paula A. Vincent

    pvincent@fbqf.unt.edu.ar

    Affiliation Departamento de Bioquímica de la Nutrición, INSIBIO (Consejo Nacional de Investigaciones Científicas y Técnicas-Universidad Nacional de Tucumán) San Miguel de Tucumán, Tucumán, Argentina

The Alternative Role of Enterobactin as an Oxidative Stress Protector Allows Escherichia coli Colony Development

  • Conrado Adler, 
  • Natalia S. Corbalan, 
  • Daiana R. Peralta, 
  • María Fernanda Pomares, 
  • Ricardo E. de Cristóbal, 
  • Paula A. Vincent
PLOS
x

Abstract

Numerous bacteria have evolved different iron uptake systems with the ability to make use of their own and heterologous siderophores. However, there is growing evidence attributing alternative roles for siderophores that might explain the potential adaptive advantages of microorganisms having multiple siderophore systems. In this work, we show the requirement of the siderophore enterobactin for Escherichia coli colony development in minimal media. We observed that a strain impaired in enterobactin production (entE mutant) was unable to form colonies on M9 agar medium meanwhile its growth was normal on LB agar medium. Given that, neither iron nor citrate supplementation restored colony growth, the role of enterobactin as an iron uptake-facilitator would not explain its requirement for colony development. The absence of colony development was reverted either by addition of enterobactin, the reducing agent ascorbic acid or by incubating in anaerobic culture conditions with no additives. Then, we associated the enterobactin requirement for colony development with its ability to reduce oxidative stress, which we found to be higher in media where the colony development was impaired (M9) compared with media where the strain was able to form colonies (LB). Since oxyR and soxS mutants (two major stress response regulators) formed colonies in M9 agar medium, we hypothesize that enterobactin could be an important piece in the oxidative stress response repertoire, particularly required in the context of colony formation. In addition, we show that enterobactin has to be hydrolyzed after reaching the cell cytoplasm in order to enable colony development. By favoring iron release, hydrolysis of the enterobactin-iron complex, not only would assure covering iron needs, but would also provide the cell with a molecule with exposed hydroxyl groups (hydrolyzed enterobactin). This molecule would be able to scavenge radicals and therefore reduce oxidative stress.

Introduction

Iron is essential for every organism, and bacteria are not an exception. Iron is present in bacterial proteins as [Fe S] clusters, and in heme groups [1]. Under aerobic conditions and at physiological pH, iron is present in the Fe+3 state and forms insoluble hydroxides and oxyhydroxide precipitates [2]. To acquire iron, bacteria have developed sophisticated strategies involving the production of iron chelators termed siderophores. Once secreted to the environment, siderophores bind iron with high affinity and import it into the bacterial cytoplasm via specific membrane receptors [1][3]. In nature, there is a myriad of siderophores and they all belong to a few structural classes, including catecholate, carboxylate, hydroxamate, and mixed ligand siderophores [4]. While it is considered that all siderophores play an equivalent role, in terms of iron uptake, their structural variety suggests functional differences.

Escherichia coli synthesizes the catechol siderophore, enterobactin, along with a specific transport system [5] (Fig. S1). Enterobactin is synthesized in the cytoplasm and exported by the inner and outer membrane transporters EntS and TolC, respectively [6]. Once in the extracellular space, enterobactin chelates iron and forms a complex that interacts with the outer membrane receptor FepA. Transport through FepA towards the periplasm, requires the energy provided by the TonB-ExbB-ExbD system anchored at the inner membrane. Subsequently, the enterobactin-iron complex binds the FepB protein and then interacts with the cytoplasmic pore constituted by FepD and FepG. Next, the ATPase, FepC, facilitates the ferric-enterobactin complex import into the cytoplasm [7]. There, the complex is hydrolyzed by the esterase Fes allowing iron to be released from its coordination with enterobactin hydroxyl groups [8]. Enterobactin is the most avid microbial iron chelator (Ka = 1052) [8]. Nevertheless, it has been reported that E. coli might have up to nine iron transport systems [9][17], most of them involving siderophore-iron complexes. In addition, E. coli mutants in iron transporters are capable of internalizing iron through the zinc transporter ZupT [18]. Bacteria endowed with multiple iron uptake systems are commonplace in nature [19]. In fact, some bacteria may produce more than one siderophore and also might have the machinery to make use of siderophores produced by other bacteria [19]. This seemingly redundant scenario in terms of iron internalization could indicate that siderophores might have additional and specific functions (i.e. in adaptation to different environments). However, until now there is limited experimental evidence enclosing siderophores in alternative physiological roles beyond its known function in iron uptake.

It has been reported that siderophores may be involved in the metabolism of other metals and, specifically, to have a role in heavy metal tolerance [20][22]. Furthermore, it was reported that binding of iron-siderophore complexes to specific receptors can trigger signal transduction mechanisms, that affect the expression of genes involved not only in iron uptake [23]. In addition, a number of hydroxamate siderophores including desferrioxamine E were shown to have inhibitory growth activity or to reduce biofilm development in some species [24][27]. In line with the alternative role of siderophores, it was demonstrated that desferrioxamine E promotes antibiotic production and has a modulatory effect on the colony development within the genus Streptomyces [28]. Additional evidence connecting siderophores and bacterial growth was found through experiments in which “non-cultured” microorganisms became “cultured” in the presence of heterologous siderophores [19]. While some of the mentioned mechanisms might involve iron metabolism, it is likely the participation of other cellular components aside from those committed to covering iron requirements.

In previous work [29] we showed that the Pseudomonad siderophore pyochelin has antibiotic activity against some bacteria. We observed a differential sensitivity to pyochelin in a panel of bacteria tested where catecholate siderophore-producing strains were resistant to pyochelin, while strains producing other type of siderophores were sensitive. Further analysis allowed us to correlate the antibiotic activity of pyochelin with the generation of reactive oxygen species (ROS) and the catechol mediated protection with the ability to reduce ROS [29]. Although E. coli has many defense mechanisms against oxidative stress, our results showed that the absence of enterobactin resulted in decreased growth in the presence of a compound that generates ROS [29]. Considering the putative role of enterobactin as an oxidative stress protector, and the association of defective growth phenotypes with oxidative stress (e.g. viable but not culturable state) [30], [31], we decided to analyze the impact of enterobactin absence on E. coli growth.

In the present work, we demonstrate that enterobactin plays a critical role in E. coli colony development in a minimal medium. We show that instead of the iron uptake impairment, it is the oxidative stress associated with the absence of enterobactin a key element in preventing cells lacking the siderophore from developing colonies. Therefore, we suggest that this siderophore has an oxidative stress protection effect that would be primarily required for colony development.

Results and Discussion

The Lack of Enterobactin Affects E. coli Growth

We previously showed that a strain impaired in enterobactin biosynthesis had significantly higher levels of reactive oxygen species compared with the wild-type strain when grown in M9 medium [29]. Thus, we assigned a putative physiological role for enterobactin in reducing cell oxidative stress. Then, we wondered if the lack of enterobactin would affect cells growth as a consequence of an imbalanced response to oxidative stress. To analyze this hypothesis, we cultured entE E. coli and wild-type E. coli in liquid aerated minimal M9 medium. Interestingly, despite of not synthesizing enterobactin, the entE strain was able to grow in minimal media, at a comparable rate to that of the wild-type strain (Fig. 1A). The observed growth differences between both strains (Fig. 1A), were not as remarkable as it could be expected, considering the relatively low iron content of M9 medium (1.8 µM) [32] and that enterobactin is the most important iron uptake facilitator that E. coli has [7], [33]. In addition, when medium was supplemented with iron (100 µM), growth of the mutant strain increased and reached OD values close to those of the wild-type strain (Fig. 1A). Thus, the differential growth rate observed for the entE mutant in liquid aerated culture could be mostly attributed to the iron scavenging property of enterobactin. Nevertheless, when entE cells in stationary phase were plated in M9 agar medium (M9A) and incubated overnight for colony count, there was no growth at dilutions where colony formation was expected (Fig. 2). Unlike E. coli entE, wild-type E. coli formed colonies in the conditions used. Figure 2 shows the type of growth observed for the entE mutant and the wild-type strain after respective culture dilutions were plated on M9A and incubated overnight. The inability of entE mutant to form colonies in M9A is an interesting growth phenotype since this strain grows normally on LB agar medium (LBA) (Table 1). Table 1 describes the type of growth (lawn or isolated colonies) for the dilutions plated on different media and conditions. For entE and wild-type cultures in all conditions used we obtained lawns with 10−4 dilutions and below (Table 1). For the wild-type, colonies were observed for 10−5 dilutions and above. In contrast, the entE mutant showed no growth at these dilutions (Fig. 2 and Table 1). This meant an abrupt growth interruption for entE strain at higher dilutions and led us to inquire about the lawn thickness of both wild-type and entE strains. To address this question, we estimated the cellular densities of spots obtained after overnight incubation of 10−4 dilutions for both strains. This was done by scraping cells off each spot and subsequently counting CFU (both strains had approximately 2×109 cells, Table S1) (see material and methods section). Then, the absence of colony formation in the 10−5 dilution plates could not be attributed to the dilution effect and pointed out a defect in colony growth for the entE mutant in the culture conditions used. Similar results were observed for dilutions of exponentially growing cultures (data not shown). This indicated that this phenotype is independent from the physiological state of the plated cells. However the abrupt growth arrest at higher dilutions in the case of the entE mutant, reveals the necessity of enterobactin particularly at cellular densities that lead to colony formation. The normal growth of entE cells on LBA (Table 1) implies that the observed atypical growth on M9A depends on the culture medium composition. Given that iron addition enhanced entE growth in aerated M9 liquid cultures (Fig. 1A) and that LB iron content is significantly higher than in M9 medium (LB: 17 µM/M9: 1.8 µM) [32], we hypothesized that iron availability could be the most likely reason for the differential growth. Then, we supplemented M9A medium with an excess of iron (100 µM) and evaluated its effect on the absence of colony formation. Curiously, we observed that iron addition in either, the initial liquid M9 culture, the solid media M9A (where dilutions were plated) or both, had no effect on the colony development arrest (Table 1). In order to assess if the entE mutant strain was able to respond to iron supplementation (100 µM FeCl3) when growing in agar media, we followed its growth as a lawn on M9A and as colonies on LBA (Fig. 1B and 1C, respectively). We found that, as with the entE liquid cultures (Fig. 1A), iron supplementation in M9A made entE lawn growth similar to that of the wild-type strain growing without iron addition (Fig. 1B). The observation was made at 8 h of incubation, a time point where lawn growth differences were clearly observed. Therefore, despite that entE cells cannot form colonies in M9A, they are able to grow as a lawn and increase this type of growth upon iron addition. Furthermore, in LBA where entE is able to form colonies, iron addition increased colony size making it similar to that of the wild-type strain (Fig. 1C). Results indicate that in all culture conditions assayed, iron is available for entE cells even though they cannot synthesize enterobactin. Additional evidence of the entE strain ability to internalize iron is the repression of the fur regulated promoter rhyB (in an entE context) to levels comparable to the wild-type strain, upon medium supplementation with 100 µM FeCl3, (Fig. 1D). Taken together, these results suggest that in the absence of enterobactin, other iron uptake systems compensate for the iron requirements. Therefore, enterobactin would play in the conditions used, a critical role in colony development, a process that would not be associated with iron shortage.

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Figure 1. Growth of E. coli wild-type (wt) and entE strains in liquid and solid media.

A) Liquid aerated minimal M9 medium cultures of wild-type strain (blue squares), entE strain (green circles) and entE strain in the same media but supplemented with 100 µM FeCl3 (red triangles). Growth (OD600) was determined at the indicated times. B) Lawn growth of wt and entE E. coli strains on M9A. A stationary phase culture of entE E. coli strain was serially diluted (10−1 to 10−4) and an aliquot of these dilutions was applied on M9A or M9A supplemented with 100 µM FeCl3. As control, the same dilutions of a wt strain overnight culture were applied on M9A medium. Lawn growth was compared at 8 hours of incubation. C) Colony growth of wt and entE E. coli on LBA. A stationary phase culture of entE E. coli strain was serially diluted and an aliquot of dilutions 10−6 to 10−8 were applied on LBA or LBA supplemented with 100 µM FeCl3. As control, the same dilutions of an overnight culture of the wt strain were applied on LBA medium. After overnight incubation, colonies sizes were compared. D) Activity of the rhyB promoter estimated by β-galactosidase activity as an indirect measure of the intracellular iron content (The higher the promoter expression, the lower the iron content [48]). Both wild-type strain and entE mutant respond to iron addition. The plasmid pALM23 carries the ryhB- lacZ fusion.

http://dx.doi.org/10.1371/journal.pone.0084734.g001

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Figure 2. Observed type of growth of entE and wild-type strains in M9A after plating and overnight incubation of serial dilutions obtained from stationary phase cultures.

Representative pictures show the characteristic leap from lawn growth (10−4 dilution) to absence of colonies (10−5 dilution) for the entE strain in M9A.

http://dx.doi.org/10.1371/journal.pone.0084734.g002

Oxidative Stress in entE Cells Leads to the Inability to Form Colonies

Since we previously reported a putative role for enterobactin in reducing reactive oxygen species [29], we wondered if entE mutants’ impairment in colony formation would be connected to oxidative stress. In fact, media supplementation with the reducing agent ascorbic acid allowed entE cells to form colonies in M9A (Table 1). Consistent with the observed lawn growth at high cellular densities and no growth at low cellular densities in M9A count plates (Fig. 2), when entE strain was streaked in M9A and incubated in aerobic conditions, only lawn growth was observed (Fig. 3B). On the contrary, when it was incubated under anaerobic conditions it was able to form colonies (Fig. 3C) similar to those of the wild-type strain grown aerobically (Fig. 3A). In concordance with these results, we observed that strains able to produce enterobactin but impaired in its internalization into the cytoplasm (fepD and fepG mutants) displayed the same phenotype in aerobic culture conditions (Fig. 4A). Similarly as reported previously for entE mutants, we observed increased ROS levels for fepD and fepG mutants compared with the wild-type strain (Fig. 4B). This suggests that in order to reduce oxidative stress, enterobactin has to be internalized and reach the cell cytoplasm. Therefore, a mutant defective in enterobactin export should accumulate enterobactin, rendering it unable to use this system to internalize iron, and should be fully functional in terms of ROS scavenging. Thus, we evaluated the colony formation phenotype and the ROS levels of the entS mutant. This mutant showed a normal growth phenotype (data not shown) and as expected ROS levels were lower than those of the entE strain and similar to levels obtained with the wild-type strain (Fig. 4B). These observations allowed us to assign an oxidative stress protection effect of enterobactin that would occur in the cytoplasm and that would be primarily required for colony development. Results with entS mutant decouple the ability of enterobactin to reduce ROS from its fundamental role in iron uptake. However, in physiological conditions where enterobactin is probably exported immediately after being synthesized, enterobactin mediated ROS scavenging would likely require its internalization along with iron.

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Figure 3. Growth of E. coli wild-type and entE mutant streaked in M9A.

Wild-type strain growth in aerobic conditions (A) and entE mutant growth in aerobic (B) or anaerobic conditions (C).

http://dx.doi.org/10.1371/journal.pone.0084734.g003

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Figure 4. A) Type of growth of E. coli fepD and fepG mutants streaked in M9A and incubated overnight in aerobic conditions. B) Levels of reactive oxygen species in E. coli wild-type and fepD, fepG, entS and entE mutants grown in M9 medium. Quantitation of ROS levels was done using the DCFA-DA probe. Fluorescence intensities are relative to that of the control. Control: wt grown in M9 medium. Error bars = SD, n = 3.

http://dx.doi.org/10.1371/journal.pone.0084734.g004

Since entE mutant grew normally at high cellular densities, the ROS protection function of enterobactin would not be as critical for lawn growth (Fig. 2 and Fig. 3B). These results are in concordance with previous reports that link high cellular density with tolerance of microorganisms to adverse conditions such as antibiotics, toxic agents and oxidative stress [34], [35]. In fact, Ma & Eaton [36], demonstrated that the absence of catalase activity rendered cells particularly sensitive to hydrogen peroxide at low cellular densities, therefore implying a counterbalancing effect at high cellular densities. It remains to be evaluated the mechanism by which high cellular density of the entE mutant strain overcomes the oxidative stress to allow growth.

Medium Composition Influence on Oxidative Stress of entE Cells

We observed that the entE mutant was unable to form colonies when grown in M9A, however normal colonies were obtained in LBA. Then, we analyzed media composition in order to unravel the cause for the differential growth in both media. Since supplementation of LBA with phosphate (40 mM) did not arrest colony formation and since entE strain still showed the phenotype in a low phosphate minimum medium (MTA) (data not shown), we ruled out the high phosphate content of M9A as a cause. LBA is a much more complex and nutritious medium than M9A, therefore we hypothesized that higher nutrient availability could favor colony formation in LBA. Therefore, we evaluated the effect of increasing casamino acids content of M9A on colony growth. To our surprise, colony development was restored by increasing casamino acids content from 0.2% up to 1% (Table 1). Then, we decided to analyze whether media composition would correlate with oxidative stress levels. For that, we measured ROS levels for entE cells in standing cultures in the same media where colonies developed (LB and M9 plus 1% casamino acids) and in the medium where they did not (M9). Figure 5 shows that ROS levels are increased for entE cells grown in M9 compared with entE cells in LB or M9 with 1% of casamino acids. In addition, ROS levels for the wild-type strain grown in M9 were similar to those of the entE mutant in LB (Fig. 5). These results suggest that lowered ROS levels could be a consequence of the higher amino acid content (in LB and M9 with 1% casamino acids) which is probably reducing ROS through direct radical scavenging [37]. Then, in 0.2% casamino acids M9 medium, enterobactin would play a significant role as an oxidative stress protector that allows colony formation. Accordingly, we observed no colony development in other saline minimal medium (MTA) and normal growth in other rich media (BHI and YEM) (Data not shown).

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Figure 5. Reactive oxygen species levels in E. coli entE mutant grown in different culture media.

Quantitation of ROS levels was done using the DCFA-DA probe. Fluorescence intensities are relative to that of the control. Control: wild-type strain grown in M9 medium; entE M9: indicates cells grown in M9 medium, entE LB: indicates cells grown in LB medium, entE M9 1% cas: indicates cells grown in M9 medium supplemented with 1% casamino acids. Error bars = SD, n = 3.

http://dx.doi.org/10.1371/journal.pone.0084734.g005

Colony Formation Resumes by Reducing Oxidative Stress

Lawn growth of entE mutant and its inability to form colonies in M9A could imply that entE cells at low cellular densities enter into a physiological state where colony development is arrested. To address this hypothesis we used the following strategy: in plates in which no growth was obtained after 24 h of incubation (10−5 dilutions of an overnight culture) we spotted 1 µL of pure enterobactin (1 µM), reincubated plates and looked for colony formation. Interestingly, we observed a size gradient of colonies around the spot containing enterobactin (Fig. 6A). This physiological complementation indicated us that the absence of colony development is a reversible phenomenon and that enterobactin addition is able to restore colony growth. As was expected, ascorbic acid addition had a similar effect (Fig. 6B) and therefore strengthened the idea that oxidative stress is a key element in arresting colony development. Furthermore, casamino acids were also able to rescue entE cells from the arrest state (Fig. 6C) probably by reducing oxidative stress levels as was implied above (Fig. 5). In contrast, neither iron (20 mM) nor citrate (1 mM) addition restored colony formation (Fig. 6D–E). This is relevant since by expressing its cognate membrane receptor FecA, E. coli can use citrate as bona fide siderophore [38]. Besides, citrate-iron complexes can further augment iron uptake through the iron starvation sigma factor FecI, which increases the expression of genes involved in iron metabolism [39]. Therefore, these results support the idea that iron availability is not accountable for the impaired colony development of entE cells. Finally, since both citrate and enterobactin facilitate iron uptake, there must be a structural trait of enterobactin that is responsible for lessening the oxidative stress and therefore allows colony formation.

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Figure 6. Colonies resume growth upon enterobactin, ascorbic acid or casamino acids (cas) addition.

In plates in which no growth was obtained after overnight incubation (10−5 dilutions), 1 µL of 1 µM enterobactin (A), 5 µL of 1 mM ascorbic acid (B), 5 µL of 2% casamino acids (C), 10 µL of 1 mM FeCl3 (D) or 10 µL of 1 mM sodium citrate (E) were spotted. After a second overnight incubation, a size gradient of colonies was clearly observed around the spots containing enterobactin (A), ascorbic acid (B) and casamino acids (C). However, no growth was observed with FeCl3 (D) or citrate (E).

http://dx.doi.org/10.1371/journal.pone.0084734.g006

Enterobactin Hydrolysis would be Required for Oxidative Stress Protection

Enterobactin structure has a central triserine macrocycle linked to three lateral catecholate moieties which are involved in iron complexation [7]. Due to their low radical reduction potentials, catechols can act as hydrogen atom donors and efficiently terminate radical chain reactions [40]. This ability requires hydroxyl moieties to be available for radical scavenging [41]. Accordingly, we observed that a mutant unable to free iron from the enterobactin-iron complex (fes) did not form colonies in M9A (Fig. 7A). Furthermore, meanwhile enterobactin addition did not resume fes strain colony development, ascorbic acid did (Fig. 7B). As expected, the fes mutant showed increased ROS levels compared with the wild-type strain and enterobactin supplementation was not able to lower ROS levels, as was previously observed for the entE strain (Fig. 7C) [29]. These results indicate that enterobactin not only has to reach the cell cytoplasm (Fig. 4A) but also has to be hydrolyzed in order to allow colony development through oxidative stress protection. Since iron availability does not seem to be involved in the colony growth arrest, we hypothesize that freed hydroxyl groups in the enterobactin molecule are responsible for the oxidative stress protection. Several reports link catechol siderophores with oxidative stress. For example, Bacillus anthracis catecholate siderophores, bacillbactin and petrobactin, are overproduced when cells are exposed to oxidative stress [42]. In Azotobacter vinelandii it was demonstrated that oxidative stress increased a catecholate siderophore synthesis and that its production was under the control of SoxS [43]. We previously showed that enterobactin protects against the ROS-mediated toxic effects of pyochelin and that impairment of enterobactin biosynthesis resulted in increased ROS levels [29]. Recently, Achard et al [44] demonstrated that the catecholate siderophores salmochelin and enterobactin protect S. Typhimurium against ROS, specially at early stages of macrophage invasion which correlate with the oxidative burst. Authors also showed that non-catecholate siderophores do not exert this protection and also that catechols need to be internalized in order to fully protect Salmonella against the oxidative stress [44].

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Figure 7. A) Type of growth of E. coli fes mutant streaked in M9A and incubated overnight in aerobic conditions. B) No colony development was observed when a 10−5 dilution of a fes mutant stationary phase culture was incubated overnight. Then, 1 µL of pure enterobactin (1 µM) or 5 µL ascorbic acid (1 mM) were spotted on the medium surface and reincubated overnight. It can be observed that ascorbic acid restores colony growth of fes mutant meanwhile enterobactin does not. C) Reactive oxygen species levels in E. coli fes and entE mutants grown in M9 medium. Quantitation of ROS levels using the DCFA-DA probe. Fluorescence intensities are relative to that of the control. Control: wt strain grown in M9 medium; +ENT: indicates addition of 1 µM enterobactin. Error bars = SD, n = 3.

http://dx.doi.org/10.1371/journal.pone.0084734.g007

Therefore, it is conceivable that catechols may be employed as protectants against oxidative stress. E. coli has many mechanisms that help cells to cope with oxidative stress. Examples are those coordinated through the OxyR and SoxSR regulons [45]. However, we observed that oxyR and soxS mutants displayed a normal colony growth in conditions where the entE mutant failed to form colonies (M9A) (data not shown). Thus, we hypothesize that enterobactin would be mostly relevant in reducing oxidative stress in situations associated with low cellular densities (e.g. single cells plated to obtain isolated colonies). It is interesting to note that enterobactin hydroxyl moieties would require to be released from the coordination complex with iron, in order to protect from the oxidative stress. Then, this iron uptake system would ensure E. coli not only iron entry into the cell, which might lead to oxidative stress through Fenton reaction, but the simultaneous generation of a molecule that scavenges ROS and therefore counterbalances the potential damage that iron excess might cause.

Materials and Methods

Bacterial Strains and Growth Conditions

List of strains and plasmids used in this work are showing in Table 2.

Strains were grown in either LB (Sigma-Aldrich) and M9 (Sigma-Aldrich) medium supplemented with 0.2% or 1% casamino acids, 0.2% glucose, 1 mM MgSO4 and 1 mg/mL vitamin B1. Solid media contained 1.5% agar. For growth curves, culture aliquots were taken at different times and OD at 600 nm was measured. For the observation of the colony arrest phenotype, 100 µL of serial dilutions (made with M9 medium) from an overnight culture of either entE or wild-type strains were plated on the corresponding agar medium and incubated overnight. When indicated, ascorbic acid and FeCl3 were supplemented at a final concentration of 1 mM and 100 µM, respectively. Anaerobic cultures were performed in an anaerobic jar containing anaerobic-generating salts (Anaerocult- Merck Millipore). For the colony arrest reversion assay, 1 µL of 1 µM enterobactin (EMC micro collections), 5 µL of 1 mM ascorbic acid (Sigma- Aldrich), 5 µL of 2% casamino acids (Sigma- Aldrich), 10 µL of 1 mM FeCl3 (Sigma- Aldrich) or 10 µL of 1 mM sodium citrate (Sigma- Aldrich) were spotted on the surface of plates where no colonies were obtained after overnight incubation (10−5 dilution from entE overnight culture). To compare the cell density of lawns obtained with 10−4 dilutions of entE and wild-type overnight cultures, we used the following approach: Four 50 µL fractions of a 10−4 dilution from each culture strain (entE and wild-type) were spotted onto M9A. After 24 h of incubation each spot was scraped off and resuspended in 1 mL of M9 medium. Serial dilutions were made and CFU count was determined in LBA for quadrupled.

Measurement of Reactive Oxygen Species

To determine the level of reactive oxygen species (ROS), we used the oxidation-sensitive fluorescent dye 2′, 7′-dichlorodihydrofluorescein diacetate (DCFH-DA). This fluorescent probe is frequently used for detection of reactive oxygen species such as hydrogen peroxide, hydroxyl radical, peroxyl radicals and nitrogen radicals [46]. DCFH-DA is deacetylated by cellular esterases and then converted by reactive species into dichlorofluorescein (DCF), which can easily be visualized by strong fluorescence at 530 nm when excited at 485 nm. Exponentially growing cells in M9 minimal medium, were washed and resuspended in 50 mM sodium phosphate buffer, pH 7 at a final OD600 nm = 0.5. Then DCFH-DA was added at a final concentration of 10 mM and incubated for 30 min [28]. After incubation, cells were washed, resuspended and sonicated in the same buffer. Fluorescence intensity was measured using a Perkin Elmer LS55 spectrofluorometer (excitation λ, 490 nm; emission λ, 519 nm). Results are expressed as relative fluorescence to that of the control.

β-Galactosidase Assays

The β-galactosidase activity was determined following the method described by Zhou et al (Zhou & Gottesman, 1998 [47]). Strains carrying the ryhB-lacZ transcriptional fusion were grown in M9 medium at 37°C up to OD600 nm = 0.1, at this point the culture was divided in half and one sample was supplemented with 100 µM FeCl3. When cultures reached an OD600 nm = 0.6, the β-galactosidase activities were assayed. For this, 600 µL aliquots of these cultures were permeabilized for 10 min with 0.1% SDS (24 µL) and chloroform (48 µL). Then, 100 µL of permeabilized cells were put onto 96 wells microtiter plate, 100 µL of a 1.32 mg/mL solution of o-Nitrophenyl-β-D-galactopyranoside in buffer Z were added and absorbances at 420 nm were measured for 20 min, in a SpectraMax 250 spectrophotometer. The β-galactosidase activity was calculated by dividing the slope of the line over time by the corresponding OD600 nm.

Supporting Information

Figure S1.

Scheme of enterobactin iron uptake system.

doi:10.1371/journal.pone.0084734.s001

(TIF)

Table S1.

Comparison of cell density of spots obtained with 10−4 dilutions.

doi:10.1371/journal.pone.0084734.s002

(DOCX)

Acknowledgments

We thank Dr. Bernhardt and Dr. Payne for kindly supplying us with entS mutant and the ryhB-lacZ plasmid, respectively.

Author Contributions

Conceived and designed the experiments: CA PAV. Performed the experiments: CA NSC DRP MFP. Analyzed the data: CA NSC REDC PAV. Contributed reagents/materials/analysis tools: PAV. Wrote the paper: CA PAV.

References

  1. 1. Andrews SC, Robinson AK, Rodriguez-Quinones F (2003) Bacterial iron homeostasis. FEMS Microbiol Rev 27: 215–237.
  2. 2. Guerinot ML, Yi Y (1994) Iron: Nutritious, Noxious, and Not Readily Available. Plant Physiol 104: 815–820.
  3. 3. Wandersman C, Delepelaire P (2004) Bacterial iron sources: from siderophores to hemophores. Annu Rev Microbiol 58: 611–647.
  4. 4. Hider RC, Kong X (2010) Chemistry and biology of siderophores. Nat Prod Rep 27: 637–657.
  5. 5. Neilands JB (1982) Microbial envelope proteins related to iron. Annu Rev Microbiol 36: 285–309.
  6. 6. Bleuel C, Grosse C, Taudte N, Scherer J, Wesenberg D, et al. (2005) TolC is involved in enterobactin efflux across the outer membrane of Escherichia coli. J Bacteriol 187: 6701–6707.
  7. 7. Raymond KN, Dertz EA, Kim SS (2003) Enterobactin: an archetype for microbial iron transport. Proc Natl Acad Sci U S A 100: 3584–3588.
  8. 8. Carrano CJ, KN R (1979) Ferric Ion Sequestering Agents. 2. Kinetics and Mechanism of Iron Removal from Transferrin by Enterobactin and Synthetic Tricatechols. J Am Chem Soc 101: 5401–5404.
  9. 9. Clarke TE, Tari LW, Vogel HJ (2001) Structural biology of bacterial iron uptake systems. Curr Top Med Chem 1: 7–30.
  10. 10. Chenault SS, Earhart CF (1991) Organization of genes encoding membrane proteins of the Escherichia coli ferrienterobactin permease. Mol Microbiol 5: 1405–1413.
  11. 11. Faraldo-Gomez JD, Sansom MS (2003) Acquisition of siderophores in gram-negative bacteria. Nat Rev Mol Cell Biol 4: 105–116.
  12. 12. Kammler M, Schon C, Hantke K (1993) Characterization of the ferrous iron uptake system of Escherichia coli. J Bacteriol 175: 6212–6219.
  13. 13. Negre VL, Bonacorsi S, Schubert S, Bidet P, Nassif X, et al. (2004) The siderophore receptor IroN, but not the high-pathogenicity island or the hemin receptor ChuA, contributes to the bacteremic step of Escherichia coli neonatal meningitis. Infect Immun 72: 1216–1220.
  14. 14. Neilands JB (1992) Mechanism and regulation of synthesis of aerobactin in Escherichia coli K12 (pColV-K30). Can J Microbiol 38: 728–733.
  15. 15. Ozenberger BA, Nahlik MS, McIntosh MA (1987) Genetic organization of multiple fep genes encoding ferric enterobactin transport functions in Escherichia coli. J Bacteriol 169: 3638–3646.
  16. 16. Sorsa LJ, Dufke S, Heesemann J, Schubert S (2003) Characterization of an iroBCDEN gene cluster on a transmissible plasmid of uropathogenic Escherichia coli: evidence for horizontal transfer of a chromosomal virulence factor. Infect Immun 71: 3285–3293.
  17. 17. Torres AG, Payne SM (1997) Haem iron-transport system in enterohaemorrhagic Escherichia coli O157:H7. Mol Microbiol 23: 825–833.
  18. 18. Grass G, Franke S, Taudte N, Nies DH, Kucharski LM, et al. (2005) The metal permease ZupT from Escherichia coli is a transporter with a broad substrate spectrum. J Bacteriol 187: 1604–1611.
  19. 19. D'Onofrio A, Crawford JM, Stewart EJ, Witt K, Gavrish E, et al. (2010) Siderophores from neighboring organisms promote the growth of uncultured bacteria. Chem Biol 17: 254–264.
  20. 20. Braud A, Hannauer M, Mislin GL, Schalk IJ (2009) The Pseudomonas aeruginosa pyochelin-iron uptake pathway and its metal specificity. J Bacteriol 191: 3517–3525.
  21. 21. Schalk IJ, Hannauer M, Braud A (2011) New roles for bacterial siderophores in metal transport and tolerance. Environ Microbiol 13: 2844–2854.
  22. 22. Teitzel GM, Geddie A, De Long SK, Kirisits MJ, Whiteley M, et al. (2006) Survival and growth in the presence of elevated copper: transcriptional profiling of copper-stressed Pseudomonas aeruginosa. J Bacteriol 188: 7242–7256.
  23. 23. Markel E, Maciak C, Butcher BG, Myers CR, Stodghill P, et al. (2011) An extracytoplasmic function sigma factor-mediated cell surface signaling system in Pseudomonas syringae pv. tomato DC3000 regulates gene expression in response to heterologous siderophores. J Bacteriol 193: 5775–5783.
  24. 24. Al-Azemi A, Fielder MD, Abuknesha RA, Price RG (2011) Effects of chelating agent and environmental stresses on microbial biofilms: relevance to clinical microbiology. J Appl Microbiol 110: 1307–1313.
  25. 25. Chi Z, Wang XX, Ma ZC, Buzdar MA, Chi ZM (2011) The unique role of siderophore in marine-derived Aureobasidium pullulans HN6.2. Biometals.
  26. 26. Ishida S, Arai M, Niikawa H, Kobayashi M (2011) Inhibitory effect of cyclic trihydroxamate siderophore, desferrioxamine E, on the biofilm formation of Mycobacterium species. Biol Pharm Bull 34: 917–920.
  27. 27. Wang WL, Chi ZM, Chi Z, Li J, Wang XH (2009) Siderophore production by the marine-derived Aureobasidium pullulans and its antimicrobial activity. Bioresour Technol 100: 2639–2641.
  28. 28. Yamanaka K, Oikawa H, Ogawa HO, Hosono K, Shinmachi F, et al. (2005) Desferrioxamine E produced by Streptomyces griseus stimulates growth and development of Streptomyces tanashiensis. Microbiology 151: 2899–2905.
  29. 29. Adler C, Corbalan NS, Seyedsayamdost MR, Pomares MF, de Cristobal RE, et al. (2012) Catecholate siderophores protect bacteria from pyochelin toxicity. PLoS One 7: e46754.
  30. 30. Oliver JD (2010) Recent findings on the viable but nonculturable state in pathogenic bacteria. FEMS Microbiol Rev 34: 415–425.
  31. 31. Kong IS, Bates TC, Hulsmann A, Hassan H, Smith BE, et al. (2004) Role of catalase and oxyR in the viable but nonculturable state of Vibrio vulnificus. FEMS Microbiol Ecol 50: 133–142.
  32. 32. Abdul-Tehrani H, Hudson AJ, Chang YS, Timms AR, Hawkins C, et al. (1999) Ferritin mutants of Escherichia coli are iron deficient and growth impaired, and fur mutants are iron deficient. J Bacteriol 181: 1415–1428.
  33. 33. Albrecht-Gary AM, Crumbliss AL (1998) Coordination chemistry of siderophores: thermodynamics and kinetics of iron chelation and release. Met Ions Biol Syst 35: 239–327.
  34. 34. Hogan D, Kolter R (2002) Why are bacteria refractory to antimicrobials? Curr Opin Microbiol 5: 472–477.
  35. 35. Narten M, Rosin N, Schobert M, Tielen P (2011) Susceptibility of Pseudomonas aeruginosa Urinary Tract Isolates and Influence of Urinary Tract Conditions on Antibiotic Tolerance. Curr Microbiol.
  36. 36. Ma M, Eaton JW (1992) Multicellular oxidant defense in unicellular organisms. Proc Natl Acad Sci U S A 89: 7924–7928.
  37. 37. Pazos M, Andersen ML, Skibsted LH (2006) Amino acid and protein scavenging of radicals generated by iron/hydroperoxide system: an electron spin resonance spin trapping study. J Agric Food Chem 54: 10215–10221.
  38. 38. Braun V, Endriss F (2007) Energy-coupled outer membrane transport proteins and regulatory proteins. Biometals 20: 219–231.
  39. 39. Brooks BE, Buchanan SK (2008) Signaling mechanisms for activation of extracytoplasmic function (ECF) sigma factors. Biochim Biophys Acta 1778: 1930–1945.
  40. 40. Povie G, Villa G, Ford L, Pozzi D, Schiesser CH, et al. Role of catechol in the radical reduction of B-alkylcatecholboranes in presence of methanol. Chem Commun (Camb) 46: 803–805.
  41. 41. Jeong JM, Choi CH, Kang SK, Lee IH, Lee JY, et al. (2007) Antioxidant and chemosensitizing effects of flavonoids with hydroxy and/or methoxy groups and structure-activity relationship. J Pharm Pharm Sci 10: 537–546.
  42. 42. Lee JY, Passalacqua KD, Hanna PC, Sherman DH (2011) Regulation of petrobactin and bacillibactin biosynthesis in Bacillus anthracis under iron and oxygen variation. PloS One 6: e20777.
  43. 43. Tindale AE, Mehrotra M, Ottem D, Page WJ (2000) Dual regulation of catecholate siderophore biosynthesis in Azotobacter vinelandii by iron and oxidative stress. Microbiology 146 (Pt 7): 1617–1626.
  44. 44. Achard ME, Chen KW, Sweet MJ, Watts R, Schroder K, et al.. (2013) An antioxidant role for catecholate siderophores in Salmonella. Biochem J.
  45. 45. Storz G, Imlay JA (1999) Oxidative stress. Curr Opin Microbiol 2: 188–194.
  46. 46. Gomes A, Fernandes E, Lima JL (2005) Fluorescence probes used for detection of reactive oxygen species. J Biochem Biophys Methods 65: 45–80.
  47. 47. Zhou Y, Gottesman S (1998) Regulation of proteolysis of the stationary-phase sigma factor RpoS. J Bacteriol 180: 1154–1158.
  48. 48. Ma L, Payne SM (2012) AhpC is required for optimal production of enterobactin by Escherichia coli. J Bacteriol 194: 6748–6757.