Temporal transcriptomic response during arsenic stress in Herminiimonas arsenicoxydans
© Cleiss-Arnold et al; licensee BioMed Central Ltd. 2010
Received: 13 July 2010
Accepted: 17 December 2010
Published: 17 December 2010
Arsenic is present in numerous ecosystems and microorganisms have developed various mechanisms to live in such hostile environments. Herminiimonas arsenicoxydans, a bacterium isolated from arsenic contaminated sludge, has acquired remarkable capabilities to cope with arsenic. In particular our previous studies have suggested the existence of a temporal induction of arsenite oxidase, a key enzyme in arsenic metabolism, in the presence of As(III).
Microarrays were designed to compare gene transcription profiles under a temporal As(III) exposure. Transcriptome kinetic analysis demonstrated the existence of two phases in arsenic response. The expression of approximatively 14% of the whole genome was significantly affected by an As(III) early stress and 4% by an As(III) late exposure. The early response was characterized by arsenic resistance, oxidative stress, chaperone synthesis and sulfur metabolism. The late response was characterized by arsenic metabolism and associated mechanisms such as phosphate transport and motility. The major metabolic changes were confirmed by chemical, transcriptional, physiological and biochemical experiments. These early and late responses were defined as general stress response and specific response to As(III), respectively.
Gene expression patterns suggest that the exposure to As(III) induces an acute response to rapidly minimize the immediate effects of As(III). Upon a longer arsenic exposure, a broad metabolic response was induced. These data allowed to propose for the first time a kinetic model of the As(III) response in bacteria.
Bacteria live in changing environments and are subjected to a variety of environnmental stresses such as pH, temperature, osmolarity or heavy metals. Arsenic is found in numerous disturbed or natural ecosystems where it can exist in mutiple oxidation states, the most common being arsenite As(III) and arsenate As(V) . This metalloid is known to generate oxidative stress in cells by its capability to induce the formation of reactive oxygen species (ROS). The damages caused by ROS to lipids, proteins and DNA are likely to contribute to As toxicity [2, 3]. In addition, one property of arsenite, which indicates that it behaves like a soft metal, consists in a high reactivity with sulphydryls groups and that affects the activity of many proteins. Microorganisms have developed remarkable capabilities to cope with arsenic. The most common arsenic resistance mechanism depends on the presence on plasmid or chromosome of ars genes encoding proteins involved in the reduction and/or the efflux of the toxic element . Nevertheless, other arsenic resistance mechanisms have been described, i.e. arsenite oxidation and arsenic methylation [5, 6]. In addition, in various microbial species, arsenic stress is associated with arsenite oxidase activity, biofilm formation, motility, oxidative stress or sulfur assimilation [7, 8]. For example, the biofilm development by Thiomonas arsenivorans has been described as a physical barrier decreasing As(III) access to sessile cells . Remarkably, some organisms such as Rhizobium sp. NT-26, have evolved specific metabolic pathways allowing them to oxidize As(III) as an energy source [10, 11] or others are known to use As(V) in anaerobic respiration . In the heterotrophic prokaryote Herminiimonas arsenicoxydans, genome sequencing revealed the presence of four ars operons involved in the reduction of As(V) to As(III) and of one aoxAB operon involved in the oxidation of the most toxic form, As(III) to the less toxic form As(V) . In addition to this detoxification process, this bacterium exhibits positive chemotaxis and motility towards arsenic, and metalloid scavenging by exopolyssacharides.
The availability of the H. arsenicoxydans complete genome sequence offers an opportunity to study its physiology by functional genomic approaches . Our previous transcriptomic studies have demonstrated that a large number of genes encoding proteins involved in oxidative stress, low affinity import of phosphate or DNA repair are induced after 15 min As(III) exposure. However, no variation was found in the genes coding for arsenite oxidase, a key enzyme in arsenic response  recently shown to be subjected to a complex regulation . In addition, little is known regarding the kinetics of arsenic stress response in microorganisms. To address these processes, physiological analyses coupled with Western immunoblotting experiments and DNA microarrays were used to examine the temporal changes in transcriptome profiles during the transition from As(III) to As(V) species due to As(III) oxidation. Our work represents, to our knowledge, the first kinetic analysis of transcription pattern in bacteria exposed to arsenic, leading to propose a global model of arsenic response in H. arsenicoxydans.
Results and Discussion
Characterization of arsenic oxidoreduction kinetics
Overview of transcriptome profiles
To get insight into the mechanisms involved in arsenic response, including oxidoreduction processes, transcriptomic analyses were performed at different steps of the experimental time course. Cells were collected from cultures of H. arsenicoxydans induced 15 min (early), 6 hours (intermediary), 8 hours (late) or not with 0,66 mM As(III) (Figure 1A) or 13,3 mM As(V) (Figure 1B). These concentrations were choosen as they are far from H. arsenicoxydans MIC for As(III) or As(V), which is able to grow up to 5 mM and 100 mM of As(III) and As(V), respectively (Muller, 2007). Moreover, this concentration of As(III) had only a minor impact on growth rate and cells continued to divide immediately after its addition. Under As(V) stress, 128 genes were up-regulated and 107 genes were down-regulated in the early phase (B1) (7% of the genome). In the late phase (B2) the number of genes up-regulated (239 genes) and down-regulated (161 genes) increased (12% of the genome). Under As(III) stress, the proportion was inverted. The major shift in gene expression occured during the onset of the early phase (A1) with 214 genes up-regulated and 245 genes down-regulated under As(III) stress. This represents approximatly 14% of the genes whose expression was significantly affected by As(III). As cell growth progressed further into the late phase (A3), the number of genes up-regulated (60 genes) and down-regulated (73 genes) decreased, representing 4% of the genome. The large number of genes responding to As(III), especially in the early phase, suggests a major remodelling of cellular physiology. In addition, oxidoreduction kinetic was only observed under As(III) stress (Figure 1A and 1B), suggesting that the Aox-dependent oxidation largely predominate the Ars-dependent reduction process. This study therefore focused on the As(III) response in H. arsenicoxydans.
Hierachical clustering kinetics
i) Early phase
Our microarray analysis highlighted a set of stress responsive genes whose transcription was early affected by As(III). This phase contained the early up-regulated genes whose expression levels gradually decreased after the induction (Class I) or down-regulated genes whose expression levels gradually increased after the induction (Class II).
First, σE and several genes encoding proteins involved in the synthesis of cell envelope components were down-regulated (Class II, Figure 3B (regulatory function, protein synthesis and fatty acid)) whereas genes encoding proteins involved in transport were up-regulated (Class I, Figure 3A (transport)). The bacterial envelope is a major defense against threats from the environment. Due to its crucial importance, the integrity of the cell envelope, including the presence of outer membrane proteins (OMP), is closely monitored to ensure its functionality. The σE system is the major pathway  required for proper folding of OMPs and their turnover , phospholipids and lipopolysaccharide (LPS) biosynthesis, signal transduction and the expression of inner and outer membrane proteins . In Escherichia coli, the σE regulon is induced specifically in response to the unbalanced synthesis of outer membrane proteins  and to the misfolding of polypeptides that have been translocated across the cytoplasmic membrane . Our results suggest that both the organization (lipoproteins, peptidoglycan and LPS) and the functioning (transport, signal transduction) of the bacterial envelope may be changed in the early phase of the response to As(III).
Second, early As(III) stress strongly stimulated expression of genes encoding components of sulfur assimilation, sulfur oxidation and glutathione (GSH) biosynthesis pathways. In fact, mRNA levels of genes encoding all the enzymatic steps required for sulfate uptake, its conversion into cysteine and GSH were increased. The expression of these genes was induced about 3 to 22 fold after 15 min induction with As(III). The expression of some of these genes was down-regulated at 6 and 8 hours [Additional file 1: Supplemental Table S1, Class II]. In eukaryotic cells, As(III) exposure results in increased levels of reduced glutathione  and an As(III)-triglutathione complex has been found in human liver excreta , leading to the conclusion that GSH plays an important role in reducing As(III) toxicity. Most effects of arsenite result from its interaction with thiol groups of proteins, its iniophoretic properties and its ability to directly or indirectly generate free radicals and hence induce oxidative stress . Microorganisms have therefore developed defense mechanisms that either keep the concentration of the O2-derived radicals at acceptable levels or repair oxidative damages. In our previous proteomic experiments, oxidative stress proteins, such as KatA and SodB, were shown to be induced in response to As(III) stress in H. arsenicoxydans. Similarly, we observed in the present study a positive regulation of three genes (sodC, katA, ahpC) involved in the protection against oxidative stress. The sodC gene encodes the superoxide dismutase catalyzing the dismutation of the superoxide radical to H2O2, which is less toxic, and O2. In addition, katA and ahpC genes encoding a catalase and a peroxidase, respectively, are responsible for scarvenging endogenously produced H2O2. Finally, As(III) early exposure induced a glutaredoxin and various thioredoxin encoding transcripts [Additional file 1: Supplemental Table S1]. In H. arsenicoxydans the induction of genes encoding proteins involved in sulfate and GSH pathways suggests that GSH may play a key role in the cell defense against oxidative stress and metalloid toxicity by maintaining an intracellular reducing environment. GSH may detoxify arsenite by i) chelation and then removing of arsenite from the cell, ii) protection against oxidation caused by metals since GSH serves as the main redox buffer in the cell, and iii) binding to reactive sulfhydryl groups of proteins thereby protecting them from irreversible metalloid binding and/or oxidative damages . Thioredoxin is believed to serve as a cellular antioxidant by maintaining the intracellular redox state, which is greatly influenced by the presence or absence of intracellular ROS, by reducing disulfide bonds produced by various oxidants and by interacting with proteins by direct association or thiol reactivity. Glutaredoxin is also known as a thioltransferase and like thioredoxin possesses an active center disulphide bond. Finally, arsenic could indirectly produce ROS by inactivating catalytic iron-sulfur clusters of enzymes as it has been shown for enzymes of the deshydratase family in E. coli in the presence of copper. In this organism, iron-sulfur clusters are the primary targets of copper and the resulting damages lead to the release of iron atoms in the cell and the generation of hydroxyl radicals . All these cellular activities (GSH, catalase, peroxidase and thioredoxin-related) are thought to be part of a general set of reactions involved in the direct or indirect response to As(III)-mediated production of reactive oxygen species in H. arsenicoxydans.
Third, the adaptive responses of bacteria to sudden environmental changes, usually involve the induction of many major heat shock proteins MHSPs, including chaperones, proteases, transcriptional regulators and other structural proteins. As(III) induced the expression of several genes encoding MHSPs [Additional file 1: Supplemental Table S1]. The MHSPs play a role in repairing and preventing damages caused by an accumulation of unfolded proteins resulting from diverse environmental stresses. In agreement with this, our microarray data showed that As(III) early exposure induced the transcription of two uspA genes that might be involved in protecting bacterial cells against As(III) stress. The protein UspA has previously shown to be induced by As(III) . The expression of the universal stress protein A (UspA) is known to be induced by a large variety of stress conditions , our results show that these conditions include As(III).
Finally, arsenic resistance in H. arsenicoxydans is partially mediated by proteins encoded by three different ars operons and one aox operon . The clusters of ars genes encode an ArsR regulator, an As(III) extrusion pump ArsB/Acr3, an ArsH putative flavoprotein and one or two arsenate reductases ArsC. One of the loci contains an Acr3-type transporter, the others associate an ArsB-type transporter with ArsC reductases. ArsC is an enzyme that reduces As(V) to As(III) which can be pumped out by the ArsB or Acr3 membrane proteins. Both acr3 and arsB genes were induced in the presence of As(III). However, Acr3 mRNAs were only detected in 15 min As(III) exposed cells, which demonstrates that Acr3 is specific to the early response. Remarkably, the arsenite oxidase genes were not induced in early phase. The lack of induction of the aox genes is in agreement with the detection by HPLC-IC-AES of 100% As(III) (Figure 1).
ii) Late phase
This phase contains genes whose expression levels gradually increased (class II) or decreased (class I), after arsenic exposure. Multiple genes of cellular processes, cell envelope and metabolism (energy, intermediary, DNA...) were highly downregulated in class I (Figure 3B). Class II was characterized by the induction of several functional categories, i.e. genes involved in metabolism, regulatory functions and cellular processes (Figure 3A). These genes are suggested to be specific for the late response to As(III).
First, H. arsenicoxydans reacted to a late As(III) exposure by activating genes involved in the transport and assimilation of phosphate as well as other phosphorous compounds [Additional file 1: Supplemental Table S1]. Indeed, after late exposure, phosphate specific transporter (Pst) and phosphate inorganic transporter (Pit) were induced. Although we cannot exclude that the various genes involved in phosphate uptake were strongly induced because of a partial depletion of phophate in the medium, this induction could also result from the accumulation of As(V). Indeed, As(V) produced by the oxidation of As(III), which only occurred in late phase (Figure 1), may compete with phosphate because of their structural similarity. So, H. arsenicoxydans may preferentially transport phosphate via the specific Pst phosphate transport system rather than the Pit general transport mechanism, in order to reduce the entry of As(V). These observations suggest that a complex regulation of the pst and pit operons allows H. arsenicoxydans to maintain its intracellular phosphate level despite the accumulation of As(V). This further supports our previous hypothesis on the physiological link between arsenic and phosphate metabolism .
Second, genes involved in chemotactic machinery and flagellum assembly were up-regulated after late exposure to As(III). Our results from the microarray experiments during exposure to As(III) combined to previous observations  clearly demonstrate that the chemotactic response is induced by As(III). In H. arsenicoxydans the flagellar machinery is organized in a mixed peritrichous/polar cascade which is most probably synthesized through sequential hierarchy of gene activation events initiated by the expression of the master transcriptional regulator FlhDC . The microarray results strongly suggest that motility is gradually induced in response to As(III) in H. arsenicoxydans.
Finally, the aox operon was induced after late exposure. The aox operon contains aoxA encoding the small subunit of arsenite oxidase, aoxB encoding the large subunit, aoxC encoding a nitroreductase and aoxD encoding a cytochrome c552. The aoxRS operon is involved in the regulation of aoxABCD operon . All of them were induced by late As(III) stress [Additional file 1: Supplemental Table S1, Class II], which strongly suggests that arsenite oxidase activity is specific to late exposure.
Transcriptional and physiological analysis of the major metabolic changes
Our microarray data suggest that several genes play a major role in the transition from the absence of As(III) to early or late arsenic exposure. To confirm this hypothesis, chemical, transcriptional, physiological and biochemical experiments were performed.
First, to further support the involvement of glutathione synthesis and sulfate metabolism in early As(III) response (early phase) in H. arsenicoxydans, we performed quantitative RT-PCR experiments. Transcripts abundance of gloA and soxC were compared to two internal controls, i.e the putative RNA methyltransferase gene and the peptide deformylase gene, in cultures challenged 15 min, 8 hours or not by As(III). The expression of soxC and gloA mRNA was increased by a 312 and 7 fold factor, respectively, after 15 min As(III) exposure. No such induction was observed in late exposure.
To address the possible role of As(III) in the GSH pathway, the total content of GSH was measured. The pool of GSH increased after 15 min (~3 fold) and further rose over time (5 fold after 6 hours). After 8 hours the level remained unchanged, as compared with 6 hours. These observations suggest that the accumulation of GSH in response to As(III) was specific to the early phase. In addition, although we did not observed any change in the extracellular concentration of sulfate, genes encoding sulfate uptake were up-regulated after 15 min and down regulated after 6 and 8 hours [Additional file 1: Supplemental Table S1]. Moreover, genes involved in the sulfur oxidation pathway, i.e. soxC, soxD, were also induced [Additional file 1: Supplemental Table S1]. A similar induction of enzymes involved in sulfur metabolism has already been shown under oxidative stress in Pseudomonas aeruginosa. Oxidative stress enzymes, i.e. thioredoxin and superoxide dismutase, are known to be implicated in sulfur assimilation and metabolism [27, 28]. Our results suggest that the intracellular concentration of different species of sulfur compounds is altered in H. arsenicoxydans under arsenic stress, demonstrating for the first time that sulfur metabolism is also impaired in response to arsenic stress.
On the other hand, to confirm the oxidative stress response resulting from arsenic exposure, peroxidase activity was measured from cultures induced or not, 15 min, 6, 8 hours with As(III). The activity was induced 5 fold after 15 min and remained unchanged after late exposure. This observation demonstrates that peroxidase activity is also specific to the early exposure to As(III).
Similarly, to support the effect of arsenic on flagellar motility and phosphate transport in the late phase, the transcript abundance of fliC and pstSb was measured. pstSb mRNAs increased by a 455 fold factor after 8 hours As(III) exposure but no such induction was observed in early exposure. Remarkably, fliC was induced by a 14 and 11 fold change after 15 min and 8 hours, respectively.
The early response is characterized by the induction of genes involved in general stress. First, GSH is a protagonist of the primary cellular responses to As(III). The genes encoding enzymes involved in sulfate uptake (A), sulfur oxidation (B), cysteine synthesis (C) leading to cysteine containing proteins and their conversion in GSH (D) were induced. As(III)-exposed cells may thus channel a large part of the assimilated sulfur into GSH for metal chelation, cellular redox buffering and possibly also protein glutathionylation. As(III) may react with GSH to form an As(SG)3 complex (E). Interactions of these As-thiol group non specific complexes with molecular oxygen lead to the formation of reactive oxygen species such as H2O2, resulting in oxidative stress within the cell. The As(III) is extruded by ArsB or Acr3 (F) and Acr3 induction was demonstrated to be specific to early exposure. The mechanism proposed here is in agreement with the observations made with HPLC-ICP-AES, showing that no oxidation occurred in early As(III) stress and only As(III) species was present.
The late response was characterized by the induction of genes specific for arsenic. Indeed, the GSH response is downregulated (A) and the transcripts encoding arsenic resistance (B), especially arsenite oxidase and its regulation (aoxRS) (C, D), and associated mechanisms such as phosphate uptake (E) and flagellum biosynthesis (F) were upregulated. The arsenite oxidase catalyses the oxidation of As(III) in As(V) (D). As(V) may directly enter the cell via the Pst or Pit transporter (E), where it is reduced to As(III) by the arsenate reductase and extruded into the periplasm via ArsB (F). Then As(V) produced by the oxidation of As(III) is extruded out of the cell (G). The mechanism proposed here for the late response to As(III) is in agreement with the oxidoreduction kinetics and underlies the links between arsenic, phosphate and motility.
In this study, we demonstrated that the detoxification and metabolism processes are gradually expressed in H. arsenicoxydans to adapt to arsenic-rich environments. In bacteria, the response to As(III) seems therefore to be characterized by a stereotypic just-in-time transcription of specific metabolic pathways, resulting in a two-step response.
Bacterial strains and growth media
H. arsenicoxydans ULPAs1 was grown in a chemically defined medium (CDM), supplemented by 2% agar when required . Tryptone swarm plates containing CDM supplemented with 1% Bacto-Tryptone and 0.25% agar were used to assess bacterial motility.
Arsenic speciation and sulfate determination
H. arsenicoxydans was grown in CDM medium and cultures were induced when required by addition of 0.66 mM As(III) for 15 min, 1 hour, 2, 4, 6 or 8 hours. Similarly, cultures were induced or not for 15 min, 6 hours, 8 hours with 13.3 mM As(V). Culture supernatants were filtered through sterile 0,22 μm pore size filters (VWR). Arsenic species were separated by high-performance liquid chromatography (HPLC) and quantified by inductively coupled plasma-atomic emission spectrometry (ICP-AES), as previously described . Sulfate extracellular concentration was determined by ion chromatography (IC) using a Metrohm Compact IC 761 system. The column used was a MetrosepA SUPP 1-250 (4.6+250 mm) with an eluent concentration of 3 mM sodium carbonate.
Peroxidase and total glutathione assay
Peroxidase activity and total glutathione were measured from serially diluted (100-10-3) 48 hours-old cultures of H. arsenicoxydans exposed or not to As(III). The peroxidase activity was determined using the Amplex Red Hydrogen Peroxide Assay kit (Invitrogen) and the total glutathione concentration was measured using the colorimetric glutahione detection kit (PromoKine). This assay was performed according to the protocol provided by the manufacturer.
Preparation of protein extracts, SDS-PAGE separation
Protein extracts and Western immunoblotting experiments were performed as described previously in Koechler et al.
Strains were grown at 25°C for 24 hours (OD = 0,15 at 600 nm, corresponding to log-phase cells) and cultures were induced or not by addition of 0,66 mM As(III) for 15 min, 6 hours or 8 hours before extraction. After 8 hours induction the OD was checked and was still corresponding to log-phase cells (OD = 0,56). Similarly, 13,3 mM As(V) were added or not to a 24 hours cultures during 15 min, 6 hours or 8 hours. Samples were harvested and stored at - 80°C. RNA were extracted as previously described . After extraction procedure, RNA integrity was checked by electrophoregram analysis on a BioAnalyser (Agilent) and total RNA concentration was determined spectrophotometrically with a Nanodrop.
Microarrays and data analysis
Microarrays containing 60-mer oligonucleotides for all predicted H. arsenicoxydans genes http://www.genoscope.cns.fr/agc/mage/arsenoscope were used, as previously described . Briefly, total RNA (5 μg) was reverse transcribed and indirectly labelled and next hybridized to the arrays. Three distinct biological RNA samples were prepared from each growth condition at different time after induction with As(III) or As(V) (0 min and after 15 min, 6 hours or 8 hours) and labelled either by Cy3 or Cy5 in a dye-swap design. Microarray data were deposited in ArrayExpress (accession E-MEXP-2809). Scanning, data normalization and statistical analysis was performed as described . Genes showing a valid p-value and a more than two-fold decreased or increased expression were considered as differentially expressed between the conditions tested and were retained for further study.
Clustering analysis was performed using ArrayMiner http://www.optimaldesign.com/ V. 5.3.4 with the Gaussian clustering and Pearson correlation options selected. The data table included log2 ratios at three different time points (15 min, 6 and 8 hours) with t = 0 being a reference. 2349 genes were significantly up- or down-regulated in at least one of the three time points. The number of classes has to be tuned prior to the run. It was chosen to 20, as it appeared to provide homogeneous profiles within classes with a reasonable number of unclassified genes.
Quantitative real time PCR
Quantitative PCR experiments were performed as described by Koechler et al., with the following modification of thermocycling conditions: 5 min at 95°c and 40 cycles of 15 s at 95°C, 15 s at 60°c and 1 min at 72°C. Two biological replicates (independent cultures) and two quantitative PCR replicates were performed in each experience. Amplification products were designed in order to obtain less than 175 bp fragments. The pairs of primers used are listed in Additional file 1: Supplemental Table S1.
JCA was supported by a grant from the French Ministry of Education and Research. Financial support came from the Centre National de la Recherche Scientifique, the Agence Nationale de la Recherche (ANR 07-BLAN-0118 project) and the Université de Strasbourg. This work was done in the frame of the Groupement de Recherche (GDR2909-CNRS): « Métabolisme de l'Arsenic chez les Micro-organismes».
- Cullen WR, Reimer KJ: Arsenic speciation in the environment. Chemical Reviews. 1989, 89 (4): 713-764. 10.1021/cr00094a002.View ArticleGoogle Scholar
- Abernathy CO, Liu YP, Longfellow D, Aposhian HV, Beck B, Fowler B, Goyer R, Menzer R, Rossman T, Thompson C, et al: Meeting on Arsenic: Health Effects, Mechanisms of Actions, and Research Issues, Hunt Valley, Maryland, 22-24 September 1997. Environmental Health Perspectives. 1999, 107 (7): 593-597. 10.1289/ehp.99107593.PubMed CentralPubMedView ArticleGoogle Scholar
- Mandal BK, Suzuki KT: Arsenic round the world: A review. Talanta. 2002, 58 (1): 201-235. 10.1016/S0039-9140(02)00268-0.PubMedView ArticleGoogle Scholar
- Rosen BP: Biochemistry of arsenic detoxification. FEBS Letters. 2002, 529 (1): 86-92. 10.1016/S0014-5793(02)03186-1.PubMedView ArticleGoogle Scholar
- Muller D, Lièvremont D, Simeonova DD, Hubert JC, Lett MC: Arsenite oxidase aox genes from a metal-resistant beta-proteobacterium. Journal of Bacteriology. 2003, 185 (1): 135-141. 10.1128/JB.185.1.135-141.2003.PubMed CentralPubMedView ArticleGoogle Scholar
- Qin J, Rosen BP, Zhang Y, Wang G, Franke S, Rensing C: Arsenic detoxification and evolution of trimethylarsine gas by a microbial arsenite S-adenosylmethionine methyltransferase. Proceedings of the National Academy of Sciences of the United States of America. 2006, 103 (7): 2075-2080. 10.1073/pnas.0506836103.PubMed CentralPubMedView ArticleGoogle Scholar
- Thorsen M, Lagniel G, Kristiansson E, Junot C, Nerman O, Labarre J, Tamos MJ: Quantitative transcriptome, proteome, and sulfur metabolite profiling of the Saccharomyces cerevisiae response to arsenite. Physiological Genomics. 2007, 30 (1): 35-43. 10.1152/physiolgenomics.00236.2006.PubMedView ArticleGoogle Scholar
- Parvatiyar K, Alsabbagh EM, Ochsner UA, Stegemeyer MA, Smulian AG, Hwang SH, Jackson CR, McDermott TR, Hassett DJ: Global analysis of cellular factors and responses involved in Pseudomonas aeruginosa resistance to arsenite. Journal of Bacteriology. 2005, 187 (14): 4853-4864. 10.1128/JB.187.14.4853-4864.2005.PubMed CentralPubMedView ArticleGoogle Scholar
- Michel C, Jean M, Coulon S, Dictor MC, Delorme F, Morin D, Garrido F: Biofilms of As(III)-oxidising bacteria: formation and activity studies for bioremediation process development. Applied Microbiology and Biotechnology. 2007, 77 (2): 457-467. 10.1007/s00253-007-1169-4.PubMedView ArticleGoogle Scholar
- Santini JM, Sly LI, Schnagl RD, Macy JM: A new chemolithoautotrophic arsenite-oxidizing bacterium isolated from a gold mine: Phylogenetic, physiological, and preliminary biochemical studies. Applied and Environmental Microbiology. 2000, 66 (1): 92-97. 10.1128/AEM.66.1.92-97.2000.PubMed CentralPubMedView ArticleGoogle Scholar
- Santini JM, Kappler U, Ward SA, Honeychurch MJ, vanden Hoven RN, Bernhardt PV: The NT-26 cytochrome c552 and its role in arsenite oxidation. Biochimica et Biophysica Acta - Bioenergetics. 2007, 1767 (2): 189-196. 10.1016/j.bbabio.2007.01.009.View ArticleGoogle Scholar
- Stolz JF, Oremland RS: Bacterial respiration of arsenic and selenium. FEMS Microbiology Reviews. 1999, 23 (5): 615-627. 10.1111/j.1574-6976.1999.tb00416.x.PubMedView ArticleGoogle Scholar
- Muller D, Medigue C, Koechler S, Barbe V, Barakat M, Talla E, Bonnefoy V, Krin E, Arsene-Ploetze F, Carapito C: A tale of two oxidation states: bacterial colonization of arsenic-rich environments. PLoS genetics. 2007, 3 (4): 10.1371/journal.pgen.0030053.Google Scholar
- Weiss S, Carapito C, Cleiss J, Koechler S, Turlin E, Coppee JY, Heymann M, Kugler V, Stauffert M, Cruveiller S, et al: Enhanced structural and functional genome elucidation of the arsenite-oxidizing strain Herminiimonas arsenicoxydans by proteomics data. Biochimie. 2009, 91 (2): 192-203. 10.1016/j.biochi.2008.07.013.PubMedView ArticleGoogle Scholar
- Koechler S, Cleiss-Arnold J, Proux C, Sismeiro O, Dillies M-A, Goulhen-Chollet F, Hommais F, Lièvremont D, Arsène-Ploetze D, Coppée J-Y, et al: Multiple controls affect arsenite oxidase gene expression in Herminiimonas arsenicoxydans. BMC Microbiology. 2010, 10: 53-10.1186/1471-2180-10-53.PubMed CentralPubMedView ArticleGoogle Scholar
- Brooks BE, Buchanan SK: Signaling mechanisms for activation of extracytoplasmic function (ECF) sigma factors. Biochimica et Biophysica Acta - Biomembranes. 2008, 1778 (9): 1930-1945. 10.1016/j.bbamem.2007.06.005.View ArticleGoogle Scholar
- Mecsas J, Rouviere PE, Erickson JW, Donohue TJ, Gross CA: The activity of σ(E), an Escherichia coli heat-inducible σ-factor, is modulated by expression of outer membrane proteins. Genes and Development. 1993, 7 (12 B): 2618-2628. 10.1101/gad.7.12b.2618.PubMedView ArticleGoogle Scholar
- Rezuchova B, Miticka H, Homerova D, Roberts M, Kormanec J: New members of the Escherichia coli σE regulon identified by a two-plasmid system. FEMS Microbiology Letters. 2003, 225 (1): 1-7. 10.1016/S0378-1097(03)00480-4.PubMedView ArticleGoogle Scholar
- Missiakas D, Betton JM, Raina S: New components of protein folding in extracytoplasmic compartments of Escherichia coli SurA, FkpA and Skp/OmpH. Molecular Microbiology. 1996, 21 (4): 871-884. 10.1046/j.1365-2958.1996.561412.x.PubMedView ArticleGoogle Scholar
- Ochi T: Arsenic compound-induced increases in glutathione levels in cultured Chinese hamster V79 cells and mechanisms associated with changes in γ-glutamylcysteine synthetase activity, cystine uptake and utilization of cysteine. Archives of Toxicology. 1997, 71 (12): 730-740. 10.1007/s002040050454.PubMedView ArticleGoogle Scholar
- Kala SV, Neely MW, Kala G, Prater CI, Atwood DW, Rice JS, Lieberman MW: The MRP2/cMOAT transporter and arsenic-glutathione complex formation are required for biliary excretion of arsenic. Journal of Biological Chemistry. 2000, 275 (43): 33404-33408. 10.1074/jbc.M007030200.PubMedView ArticleGoogle Scholar
- Bernstam L, Nriagu J: Molecular aspects of arsenic stress. Journal of Toxicology and Environmental Health - Part B: Critical Reviews. 2000, 3 (4): 293-322. 10.1080/109374000436355.View ArticleGoogle Scholar
- Pompella A, Visvikis A, Paolicchi A, De Tata V, Casini AF: The changing faces of glutathione, a cellular protagonist. Biochemical Pharmacology. 2003, 66 (8): 1499-1503. 10.1016/S0006-2952(03)00504-5.PubMedView ArticleGoogle Scholar
- Macomber L, Imlay JA: The iron-sulfur clusters of dehydratases are primary intracellular targets of copper toxicity. Proceedings of the National Academy of Sciences of the United States of America. 2009, 106 (20): 8344-8349. 10.1073/pnas.0812808106.PubMed CentralPubMedView ArticleGoogle Scholar
- Kvint K, Nachin L, Diez A, Nyström T: The bacterial universal stress protein: Function and regulation. Current Opinion in Microbiology. 2003, 6 (2): 140-145. 10.1016/S1369-5274(03)00025-0.PubMedView ArticleGoogle Scholar
- Salunkhe P, Töpfer T, Buer J, Tümmler B: Genome-wide transcriptional profiling of the steady-state response of Pseudomonas aeruginosa to hydrogen peroxide. Journal of Bacteriology. 2005, 187 (8): 2565-2572. 10.1128/JB.187.8.2565-2572.2005.PubMed CentralPubMedView ArticleGoogle Scholar
- Zeller T, Klug G: Thioredoxins in bacteria: Functions in oxidative stress response and regulation of thioredoxin genes. Naturwissenschaften. 2006, 93 (6): 259-266. 10.1007/s00114-006-0106-1.PubMedView ArticleGoogle Scholar
- Imlay JA: Cellular defenses against superoxide and hydrogen peroxide. Annual Review of Biochemestry. 2008, 77: 755-776. 10.1146/annurev.biochem.77.061606.161055.View ArticleGoogle Scholar
- Kashyap DR, Botero LM, Franck WL, Hassett DJ, McDermott TR: Complex regulation of arsenite oxidation in Agrobacterium tumefaciens. Journal of Bacteriology. 2006, 188 (3): 1081-1088. 10.1128/JB.188.3.1081-1088.2006.PubMed CentralPubMedView ArticleGoogle Scholar
- Chevance FFV, Hughes KT: Coordinating assembly of a bacterial macromolecular machine. Nature Reviews Microbiology. 2008, 6 (6): 455-465. 10.1038/nrmicro1887.PubMedView ArticleGoogle Scholar
- Ellis PJ, Conrads T, Hille R, Kuhn P: Crystal structure of the 100 kDa arsenite oxidase from Alcaligenes faecalis in two crystal forms at 1.64 Â and 2.03 Â. Structure. 2001, 9 (2): 125-132. 10.1016/S0969-2126(01)00566-4.PubMedView ArticleGoogle Scholar
- Kashyap DR, Botero LM, Lehr C, Hassett DJ, McDermott TR: A Na+:H+ antiporter and a molybdate transporter are essential for arsenite oxidation in Agrobacterium tumefaciens. Journal of Bacteriology. 2006, 188 (4): 1577-1584. 10.1128/JB.188.4.1577-1584.2006.PubMed CentralPubMedView ArticleGoogle Scholar
- Yorimitsu T, Homma M: Na+-driven flagellar motor of Vibrio. Biochimica et Biophysica Acta - Bioenergetics. 2001, 1505 (1): 82-93. 10.1016/S0005-2728(00)00279-6.View ArticleGoogle Scholar
- Muller D, Simeonova DD, Riegel P, Mangenot S, Koechler S, Lièvremont D, Bertin PN, Lett MC: Herminiimonas arsenicoxydans sp. nov., a metalloresistant bacterium. International Journal of Systematic and Evolutionary Microbiology. 2006, 56 (8): 1765-1769. 10.1099/ijs.0.64308-0.PubMedView ArticleGoogle Scholar
- Muller D, Lievremont D, Simeonova DD, Hubert JC, Lett MC: Arsenite oxidase aox genes from a metal-resistant beta-proteobacterium. Journal of Bacteriology. 2003, 185 (1): 135-141. 10.1128/JB.185.1.135-141.2003.PubMed CentralPubMedView ArticleGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (<url>http://creativecommons.org/licenses/by/2.0</url>), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.