Research Article | Open Access
Antonia Y. Tetteh, Katherine H. Sun, Chiu-Yueh Hung, Farooqahmed S. Kittur, Gordon C. Ibeanu, Daniel Williams, Jiahua Xie, "Transcriptional Response of Selenopolypeptide Genes and Selenocysteine Biosynthesis Machinery Genes in Escherichia coli during Selenite Reduction", International Journal of Microbiology, vol. 2014, Article ID 394835, 11 pages, 2014. https://doi.org/10.1155/2014/394835
Transcriptional Response of Selenopolypeptide Genes and Selenocysteine Biosynthesis Machinery Genes in Escherichia coli during Selenite Reduction
Bacteria can reduce toxic selenite into less toxic, elemental selenium (Se0), but the mechanism on how bacterial cells reduce selenite at molecular level is still not clear. We used Escherichia coli strain K12, a common bacterial strain, as a model to study its growth response to sodium selenite (Na2SeO3) treatment and then used quantitative real-time PCR (qRT-PCR) to quantify transcript levels of three E. coli selenopolypeptide genes and a set of machinery genes for selenocysteine (SeCys) biosynthesis and incorporation into polypeptides, whose involvements in the selenite reduction are largely unknown. We determined that 5 mM Na2SeO3 treatment inhibited growth by ∼50% while 0.001 to 0.01 mM treatments stimulated cell growth by ∼30%. Under 50% inhibitory or 30% stimulatory Na2SeO3 concentration, selenopolypeptide genes (fdnG, fdoG, and fdhF) whose products require SeCys but not SeCys biosynthesis machinery genes were found to be induced ≥2-fold. In addition, one sulfur (S) metabolic gene iscS and two previously reported selenite-responsive genes sodA and gutS were also induced ≥2-fold under 50% inhibitory concentration. Our findings provide insight about the detoxification of selenite in E. coli via induction of these genes involved in the selenite reduction process.
Selenium (Se) is a nonmetal element with atomic number 34, which is chemically related to sulfur (S) and tellurium but rarely found in its elemental form in nature. Se is an essential micronutrient for mammals and some bacteria and a component of selenocysteine (SeCys), an amino acid used by a group of proteins [1, 2]. In Escherichia coli genome, there are three formate dehydrogenases FdhN, FdhO, and FdhH with each consisting of one selenopolypeptide requiring SeCys [3–6] for the oxidation of formate and carbon dioxide . At elevated concentrations, however, Se can be toxic [7, 8]. High Se levels are known to produce reactive oxygen species that cause DNA damage and various diseases in mammals [8, 9]. Previous studies have shown that some bacteria, unlike mammals and yeasts, can tolerate high levels of Se through the reduction of toxic selenate and selenite to an insoluble, less toxic, red Se element (Se0) [10–13]. In nature, selenate and selenite are two major types of soluble inorganic compounds. Selenite is more toxic than selenate and other forms of Se compounds . Hence, the reduction of selenite by microorganisms has a broad biological importance.
Several bacterial species including E. coli have the capacity to convert selenite to Se0 [15–27]. E. coli strains can grow in the presence of 9.2 mM selenite and efficiently metabolize selenite into Se0 . However, the detailed processes of how selenite is reduced, what molecular mechanism is utilized, and how bacterial cells respond to selenite are still unknown [13, 28] although the physiological mechanisms of selenite reduction have been studied in several species [12, 15, 26]. It is believed that selenite like selenate may enter the cells through the sulfate permease system controlled by cysA, cysU, and cysW . Selenite may also enter the cells through an alternative system, such as the sulfate transporter, because disruption of sulfate permease expression did not completely block its uptake . After entry into the cells, selenite may be reduced to selenide , followed by oxidation to Se0 . Further study on the molecular mechanism involved in selenite reduction is necessary, which will assist in understanding the detoxification of selenite.
Currently, the knowledge concerning the molecular mechanism involved in selenite reduction in E. coli is limited to four genes that have been identified to respond to sodium selenite (Na2SeO3) treatment. Three of them are oxidative stress stimulons sodA, gor, and trxB, encoding the manganese superoxide dismutase, glutathione reductase, and thioredoxin reductase, respectively, which are upregulated ≥5-fold by 2 mM Na2SeO3 treatment . The fourth gene is gutS (or called yhfC) that encodes the GutS polypeptide, a homolog of membrane transport proteins, which can be induced by 0.03–0.06 mM Na2SeO3 and 0.002 mM sodium tellurite . Microarray analysis was employed to investigate transcript changes genome-wide in Caulobacter crescentus cells treated with 0.3 mM Na2SeO3; only 12 genes were found to be upregulated about 2- to 5-fold . However, all of these genes were also induced by chromium and cadmium , suggesting that they are more likely to be general stress induced genes rather than specifically responding to selenite. No homologous genes of the aforementioned four selenite-induced genes involved in oxidative stress  and membrane transport  were found to be upregulated by Na2SeO3 in C. crescentus . Therefore, in depth analysis is essential to understand whether any additional genes in bacterial genome are responsible for selenite reduction.
In E. coli, there are only three proteins FdhN, FdhO, and FdhH that each contains one polypeptide requiring SeCys residue for their activities [3–6]. The gene fdnG encodes a 110 kD selenopolypeptide, subunit of FdhN. The fdoG encodes another 110 kD selenopolypeptide for FdhO while the fdhF encodes a 80 kD selenopolypeptide of FdhH. In addition, there is a group of SeCys biosynthesis and incorporation machinery genes for the biosynthesis of SeCys and selenopolypeptides such as selA (selenocysteine synthase), selB (selenocysteinyl-tRNA-specific translation factor), selC (tRNA specific for selenocysteine), selD (selenophosphate synthase) [6, 33], ybbB (selenophosphate-dependent tRNA 2-selenouridine synthase) , and sufS (PLP-dependent selenocysteine lyase) . We questioned how these genes respond during selenite reduction. To evaluate the changes in transcript levels of Se metabolic genes, Na2SeO3 concentrations that are 30% stimulatory and 50% inhibitory on bacterial cell growth were determined and used to study their expressions by quantitative real-time PCR (qRT-PCR). In addition, microarray analysis was also used to screen selenite-responsive genes besides above selected genes.
2. Materials and Methods
2.1. Bacterial Strain and Growth Conditions
E. coli strain K12 was used in this study. Bacterial cells were grown in Luria-Bertani (LB) medium in 14-mL polystyrene round-bottom tubes. A final volume of 3 mL was used for cultures and incubated at 37°C in a rotary shaker at 225 rpm for different periods of time depending on the experiment.
2.2. Screening Inhibitory and Stimulatory Concentrations
To determine which concentrations of Na2SeO3 inhibited and stimulated bacterial growth, an overnight culture of K12 adjusted to the optical density at 600 nm (OD600) of 1 was used as bacterial stock solution for testing. Na2SeO3 (Sigma-Aldrich) was dissolved in ddH2O to prepare 1 M selenite stock solution. Initially, each 20 μL of bacterial stock solution was inoculated into 3 mL LB medium containing Na2SeO3 with a final concentration of 0, 25, 50, 75, 100, or 125 mM. The experiment was performed on three biological replicates in triplicate for each concentration tested. After 14 h of growth, the extent of selenite to Se0 reduction as indicated by the degree of red color in each culture was determined qualitatively and photographs were compared. Since reduced red Se0 can interfere with optical density measurements, bacterial growth was determined by counting viable cell numbers. Cells were diluted using LB medium and then 20 μL of diluted culture was spread onto a LB agar and incubated at 37°C overnight. The serial dilutions were done in triplicate for each culture. Thus, the colony-forming units (CFUs) were calculated from nine plates for each treatment.
After the initial test, 0, 5, 10, 15, 20, 25, and 30 mM Na2SeO3 were used to determine the concentration that would inhibit the bacterial growth. Another experiment using lower concentrations (0, 0.0001, 0.001, 0.01, 0.05, 0.1, 0.5, 1, 5, and 10 mM) was performed to determine which concentration stimulated bacterial growth. Both experiments were performed on three biological replicates in triplicate for each concentration tested.
2.3. Determining a Time Point of Significant Growth Difference between 5 mM Na2SeO3 Treated and Untreated Cultures
After screening the inhibitory selenite concentration, cultures were treated with selected 5 mM Na2SeO3 to determine when cells should be harvested for RNA extraction at which significant difference in bacterial growth between treated and untreated control could be observed. The same culture conditions were used as previously mentioned; treated and untreated cultures were incubated at 37°C for 0, 2, 4, 6, 8, 10, 12, or 14 h. Colony forming units were recorded as previously mentioned for each time point. Three biological replicates done in triplicate were done for each culture.
2.4. Preparing 0.5- and 2-h Cultures for qRT-PCR Analysis
To study the effect of culture duration on induced selenite-responsive genes, two previously reported growth times, 0.5 h [30, 32] and 2 h [30, 31], and selected 6 h were tested. To determine an optimal initial culture concentration which allows cells to reach log phase of growth after 0.5 and 2 h short culture periods, cells were precultured to first reach OD600 of 0.2, 0.4, and 0.8; then, these were served as initial inoculant concentrations for culturing for 0.5, 1, 1.5, 2, 2.5, and 3 h. The cell density of each culture was recorded by measuring OD600 value. Three biological replicates with triplicate assay for each time point were done for the entire experiment.
2.5. RNA Isolation
Total RNA was isolated using the RiboPure-Bacteria RNA Isolation Kit (Applied Biosystems/Ambion, USA) and treated with DNase I (Applied Biosystems/Ambion, USA) to remove any DNA contamination. RNA concentration was quantified using a NanoDrop ND 1000 spectrophotometer. The quality of the RNA was visualized on a 1.2% agarose gel. For microarray analysis, RNA quality was further checked using a dual beam spectrophotometer and an Agilent Bioanalyzer 2100 Lab-on-a-Chip system.
2.6. qRT-PCR Analysis
Three selenopolypeptide genes (fdnG, fdoG, and fdhF) and five machinery genes (selA, selB, selD, ybbE, and sufS) for SeCys biosynthesis and insertion were selected to quantify their expression levels in response to selenite treatments. The selC was not selected because its sequence (95 bp) is too short to meet the requirement of primer design software Primer Express 3.0 (Applied Biosystems/Ambion, USA) for designing a pair of primers. Previously reported four selenite-induced genes (gor, sodA, trxB, and gutS) [30, 31] and three S metabolism related genes (sbp, sulfate transporter subunit, thiP, thiamine transporter membrane protein, and iscS, cysteine desulfurase) [36–38] were included for comparison. Bacterial cells untreated and treated either with 0.01 or 5 mM Na2SeO3 were used for RNA isolation. Equal amounts of RNA for each sample were used to synthesize first-strand of cDNA with a High Capacity cDNA Reverse Transcription kit and random primers (Applied Biosystems, USA). PCR was carried out with the Power SYBR Green mix (Applied Biosystems, USA). Primer design and ΔΔCt calculation were carried out as described previously . Sequences of selected genes were retrieved from strain K12 genome (accession no. AC_000091) deposited in NCBI (http://www.ncbi.nlm.nih.gov/) for designing primers. The 16S rRNA was used as an endogenous control. 16S rRNA primers were designed based on 719 bp conserved region of seven members (rrsA, B, C, D, E, G, and H) also retrieved from strain K12 genome. Each sample was assayed in triplicate and the experiment was repeated with three biological replicates. Detailed primer information for each gene is listed in Table 1.
2.7. Microarray Analysis
Bacterial cells untreated and treated with 0, 0.01, or 5 mM Na2SeO3 for 6 h were used for microarray analysis for screening additional selenite-responsive genes which were not in the previous qRT-PCR analysis. Three replicates for treated and untreated samples were used. The microarray chip used in this experiment was the Affymetrix GeneChip E. coli genome 2.0 arrays (Affymetrix, USA) containing 10,208 probe sets for detecting the entire 20,366 genes in the K12 strain and three other E. coli strains. The RNA quality control analysis, standardization, cRNA labeling, and array hybridization were processed at Genome Explorations Inc. (http://www.genome-explorations.com/, USA). Raw signals (CEL files) were normalized and transformed into log2 values by MAS 5 (scaled to TGT = 250). For statistical analysis, the significance analysis tool set in gene traffic was employed to perform multiclass ANOVA. Pairwise comparisons were made between untreated control and 0.01 or 5 mM treatment. All probe sets having comparisons reaching absolute fold change ≥1.5 and -test values ≤0.05 were selected for further qRT-PCR confirmation. Aforementioned qRT-PCR conditions and endogenous control were used. Sequences of related genes were retrieved from strain K12 genome. Detailed primer information for each gene is listed in Table 1.
2.8. Statistical Analysis
For the comparison of cell numbers between untreated control and Na2SeO3 treatments, Student’s -test was used.
3.1. Na2SeO3 Concentration Causing 50% Inhibitory Effects
To examine Na2SeO3 inhibitory effects on bacterial growth, E. coli K12 was cultivated in the presence of high concentration of Na2SeO3 at 0, 25, 50, 75, 100, or 125 mM. Results showed that all these selenite treatments caused more than 50% inhibition of E. coli growth (Figure 1(a)). Overnight treatment using 25 mM selenite inhibited bacterial growth about 8-fold compared to untreated cultures (Figure 1(a)) and led the culture to turn red (Figure 1(b)), indicating that selenite reduction has occurred. When 50 mM or higher selenite concentrations were used, cell numbers drastically decreased and these cultures turned slightly but not completely red. This suggests that selenite reduction was decreased under high selenite concentrations, which could be due to extremely low number of bacterial cells.
A narrower range of Na2SeO3 (0 to 30 mM with a 5 mM interval) was used to determine a concentration of Na2SeO3 that would inhibit bacterial growth by 50%. We found that 5 mM Na2SeO3 treatment reduced cell numbers by 53% and turned cultures red (Figures 1(c) and 1(d)). When concentrations of 10 to 30 mM were used, cell numbers were reduced by 79–97% and all these cultures still turned red, especially at 10 and 15 mM. These results are consistent with the previous observations that selenite can be reduced to red Se0 by E. coli [12, 30] and indicate that the selenite reduction occurred efficiently in E. coli K12 cells treated with 5 to 30 mM Na2SeO3.
3.2. Na2SeO3 Concentration Having Stimulatory Effects
Se is an essential element for bacterial growth. To determine what Na2SeO3 concentration range stimulating bacterial growth, 0 to 10 mM Na2SeO3 was tested. Compared to the untreated control, 0.0001 to 0.1 mM Na2SeO3 treatments could stimulate K12 cell growth (Figure 2(a)). The stimulatory effects were increased from 10% to 30% when the concentrations were increased from 0.0001 to 0.001 mM. However, no significant color changes were observed in 0.0001 to 0.01 mM treated cultures, indicating no or very low levels of selenite reduction occurring (Figure 2(b)). The stimulatory effects of selenite on the cell growth were decreased with increasing in Na2SeO3 concentrations (Figure 2(a)). When 0.05 to 0.5 mM treatments were used, the cultures turned red (Figure 2(b)) but the stimulatory effects of these treatments on bacterial growth were slight (Figure 2(a)). Consistently, more than 50% inhibitory effects with clear red color in cultures were observed in this experiment when Na2SeO3 concentrations reached as high as 5 and 10 mM. Based on the above results, 0.01 mM was selected as a stimulatory concentration for further studies.
3.3. Expression Levels of Selected Genes under Inhibitory and Stimulatory Conditions
To investigate how selenopolypeptide genes and machinery genes for SeCys biosynthesis and insertion respond to Na2SeO3 concentrations that cause 30% stimulatory or 50% inhibitory to bacterial cell growth, their transcript levels were quantified by qRT-PCR. For comparison, harvesting Na2SeO3-treated and untreated cultures at a time point where the most significant difference in growth is important. To this end, a ~50% inhibitory concentration of 5 mM Na2SeO3 was used for cultures and bacterial growth was monitored every 2 h for 14 h. Cell densities were significantly different between treated and untreated cultures after being grown for 2 and 4 h (Figure 3(a)). The number of cells in treated culture was reduced during the first 2 h of growth, which suggests that some cells may have died during the initial culture stage. Those survival cells gradually caught up the growth and reached the highest cell numbers at 10 h. The untreated cultures, on the other hand, reached stationary phase early at 6 h, but the highest cell numbers were also at 10 h. Therefore, 6 h was selected as a time point to harvest cells for quantifying gene expression levels.
To investigate the expression of selenite-responsive genes at different culture time point, previously reported growth times of 0.5 [30, 32] and 2 h [30, 31] were also used as well as 6 h treatment. However, the number of cells could be too low to isolate a usable quality and quantity of RNA after growing for 0.5 and 2 h if the same 20 μL bacterial stock solution (OD600 = 1) is inoculated into 3 mL LB medium. To determine which initial culture concentration would allow the culture to reach log phase after culturing for 0.5 to 3 h, a pretest culture experiment was performed with initial OD600 of 0.2, 0.4, and 0.8. The results showed that OD600 values increased from initial 0.2, 0.4, and 0.8 to 0.4, 0.6, and 0.9 after culturing for 0.5 h and to 0.9, 1.1, and 1.2 after culturing for 2 h, respectively (Figure 3(b)). Based on these observations, bacterial growths reached to log phase after 0.5 and 2 h cultures when the initial OD600 of 0.4 was used. Therefore, cultures with initial OD600 of 0.4 treated with 0.01 or 5 mM Na2SeO3 for either 0.5 or 2 h were used to study gene expression.
QRT-PCR results showed that two selenopolypeptide genes fdnG and fdoG were induced 2- to 10-fold by 0.01 or 5 mM Na2SeO3 with 2 or 6 h treatments, but not at 0.5 h (Figure 4(a)). The third one fdhF was induced about 2-fold by 0.01 and 5 mM Na2SeO3 treatments for 2 h only. The expression levels of all five SeCys biosynthesis and insertion machinery genes selA, selB, selD, ybbE, and sufS did not show ≥2-fold changes in any of the treatments (Figure 4(b)). These results suggest that maintaining the constant expression of these machinery genes is necessary for survival. Concerning three S metabolic genes, only iscS was induced 2.7- and 2.2-fold in 5 mM treatment for 2 and 6 h (Figure 4(c)). The remaining two genes in all treatments and iscS in remaining treatments did not cause ≥2-fold changes in their expression levels. When four previously reported selenite induced genes were analyzed, two of them (sodA and gutS) were induced 2.6- and 3.8-fold in 5 mM treatment for 2 and 6 h but not in the other treatments (Figure 4(d)). The expression levels of the other two genes (gor and trxB) did not meet the 2-fold cutoff under either 0.01 or 5 mM treatment, which is not in agreement with previous report by Bébien et al. .
3.4. Identification of Additional Selenite-Responsive Genes by Microarray Analysis
Microarray analysis is a powerful approach to study differential gene expression by genome-wide screening simultaneously. In order to identify genes besides above selected genes that are responsive to current selenite treatment conditions, microarray analysis was performed to compare transcript levels of genes in whole genome between untreated cells and 0.01 or 5 mM and 6 h treated cells. RNA samples from three biological replicates per treatment were used for hybridization. The results showed that average hybridization signals of probe sets were 554.4, 557.0, and 560.1 while background signals were 39.7, 45.8, and 47.4 for untreated, 0.01 mM treated, and 5 mM treated samples, respectively (Table 2). These results indicate that hybridization and scanning were efficient. After pairwise comparison of data using statistical analysis, fold changes of all genes between the untreated and 0.01 or 5 mM treated were calculated. Genome-wide comparison with 4326 genes in the K12 genome  by microarray revealed that nearly no single gene had its transcript level change more than 2-fold when cultures were grown under either 30% stimulatory or 50% inhibitory selenite conditions (data not shown). It was surprising to note that transcript levels of all above selenite-responsive genes detected by qRT-PCR did not display difference between treated and control. Only expression levels of yegB (probe set ID 1764732) were induced 2.2- and 1.8-fold by 0.01 and 5 mM treatments, respectively (Table 2), but its average hybridization signal in control group was 27.0, which is below the background signal 39.7 (Table 2).
|Selected probe sets corresponding to selenite-responsive candidate genes have absolute fold changes ≥1.5 and -test values ≤ 0.05 either in 0.01 or 5 mM Na2SeO3 treatment. bHybridization signals of average of all 10,208 probe sets and seven probe sets. Mean values ± SD . Average of background signals are 39.7 ± 2.3, 45.8 ± 1, and 47.4 ± 0.4 for 0, 0.01 and 5 mM, respectively. cFold changes of selenite-responsive candidate genes from microarray analysis comparing to untreated control. “−” means reduced expression.|
Using absolute fold change ≥1.5 and values ≤0.05 as a standard, three genes in K12 genome were induced in their expressions while two genes were inhibited by 0.01 mM Na2SeO3 treatment for 6 h (Table 2). When K12 cells were treated with 5 mM for 6 h, only two genes were induced while one was inhibited in their expressions. Among these identified selenite-responsive candidate genes, the yegB was induced ≥1.5 by both 0.01 and 5 mM treatments. However, all these candidate genes had relatively low hybridization signals (Table 2). When qRT-PCR was used to confirm expression levels of these selenite-responsive candidate genes in cells treated with 0.01 or 5 mM selenite for 0.5, 2, or 6 h, none of them had their expression level changed more than 1.5-fold under either stimulatory or inhibitory conditions (Figure 5).
Previous studies have shown that E. coli cells exhibit three types of responses when subjected to selenite treatment. At extremely low concentrations (<0.0002 mM), selenite is readily incorporated into SeCys for the synthesis of selenoproteins, such as formate dehydrogenases . At moderate concentrations (>0.001 mM), selenite intrudes the S metabolic pathway and is metabolized along the routes of S metabolism, but never affects cell growth until it reaches 0.08 mM [41, 42]. At higher concentrations (>5 mM), selenite becomes toxic via the mechanism of oxidative stress . In the present study, 0.001 to 0.01 mM sodium selenite concentrations were found to promote bacterial growth approximately by 30% (Figure 2(a)). The trend of all four concentrations used for stimulatory effect was the same although 0.001 and 0.05 mM treatments did not have significantly stimulatory effects. Meanwhile, 5 mM treatment inhibited cell growth steadily by more than 50% (Figures 1(c), 2(a), and 3(a)). The results of our growth studies are consistent with previous reports [4, 30, 41, 42] which lay a foundation for further investigating selenite-responsive genes.
Using qRT-PCR analysis, we found that all three selenopolypeptide genes fdnG, fdoG, and fdhF encoding selenopolypeptides for FdhN, FdhO, and FdhH were induced more than 2-fold by both 0.01 and 5 mM Na2SeO3 (Figure 4(a)), which have not been reported previously. E. coli has only these three proteins with each containing one selenopolypeptide requiring SeCys for its activity [3–6]. A possible role for SeCys in these enzymes could be important for the adjustment of the redox potential, making catalytic reaction possible without oxygen transfer . FdhN and FdhO are known to be responsible for the oxidation of formate and transfer of electrons from formate to nitrate [44, 45]. Therefore, observed results could be simply explained that induced expression of these genes encoding selenopolypeptides by selenite is only for the protection of bacterial cells via their antioxidation functions. This could be reasonable if fdnG, fdoG, and fdhF are only induced by 5 mM Na2SeO3 treatment. Since they were induced more than 2-fold by 0.01 mM Na2SeO3 as well, whether these proteins containing SeCys have an additional function other than antioxidation needs to be further investigated. In the presence of 0.01 mM Na2SeO3, a small part of selenite may be used to synthesize selenopolypeptides while large part may be metabolized with the S as suggested by previous studies [41, 42]. Nevertheless, these results suggest that these selenopolypeptide genes are either directly or indirectly involved in selenite reduction.
Moreover, we also found that one sulfur metabolic gene iscS and two previously reported selenite-induced genes sodA and gutS were induced only by 5 mM (Figure 4(d)), which indicate these genes are also involved in selenite reduction. Under 5 mM Na2SeO3 treatment, bacterial cells were already under toxic condition with more than 50% growth inhibition even though the selenite reduction was still active as judged from the accumulation of Se0 (Figures 1 and 2). It is known that under the toxic conditions, the reduction of selenite involves reactions with sulfhydryl groups of thiol-containing molecules, such as glutathione, and some of these reactions produce reactive oxygen species: hydrogen peroxide and superoxide [12, 30]. Both hydrogen peroxide and superoxide can cause damage to cell membranes and DNA . Therefore, the gene like sodA encoding the antioxidant enzyme  is induced in response to oxidative stress. However, it is not clear why previously reported selenite inducible genes gor and trxB, encoding antioxidant proteins glutathione reductase and thioredoxin reductase, respectively , could not be induced by selenite treatment in the present study. Induced expression of gutS by selenite was similar to the previous report . The gutS gene product may allow Se to permeate into cells because it shares homology with membrane transport proteins. Induction of iscS under the selenite toxic conditions (Figure 4(c)) may be due to its dual function in both S and Se metabolisms. Unlike the other two sulfur metabolic genes, the iscS is also required for biosynthesis of 2-selenouridine in tRNA and FdhH .
In the present study, we also made an attempt to identify selenite-responsive genes genome-wide by microarray screening. Surprisingly, this screening did not yield any selenite-responsive genes in cells treated with 50% inhibitory or 30% stimulatory Na2SeO3 concentration. Our results of microarray experiment are similar to those reported by Hu and coworkers , in which only a few general stress-induced genes were identified in their microarray screening. Although underestimation of the fold changes of differentially expressed genes in a microarray assay was reported previously in comparison with the qRT-PCR analysis , Hu and coworkers (2005)  could still use microarray analysis to identify chromium and cadmium (but not Se) induced genes in bacterium. Our current microarray results in conjunction with microarray screening results reported by Hu et al. (2005)  from selenite treated bacterial cells suggest that selenite reduction may result from minor contributions from a small set of genes with slight changes at transcript levels and that microarray analysis may not be sensitive enough to identify those selenite-responsive genes, which could be identified by qRT-PCR.
We have comprehensively studied the bacterial growth under various concentrations of Na2SeO3 and determined that 0.001 to 0.01 mM promoted bacterial growth approximately by 30%, whereas 5 mM treatment inhibited cell growth by more than 50%. Although microarray analysis was not sensitive enough to identify these selenite-responsive genes in bacteria, we were able to determine that genes encoding selenopolypeptides and some antioxidant proteins were involved in selenite reduction. Our findings will help to further elucidate the mechanism responsible for selenite reduction.
Conflict of Interests
The authors declare that there is no conflict of interests regarding the publication of this paper.
This work was supported by a United States Department of Agriculture-Cooperative State Research, Education, and Extension Service grant (no. 2009-35318-05032), a Biotechnology Research grant (no. 2007-BRG-1223) from the North Carolina Biotechnology Center, and a startup fund from the Golden LEAF Foundation to the Biomanufacturing Research Institute and Technology Enterprise (BRITE).
- M. Birringer, S. Pilawa, and L. Flohé, “Trends in selenium biochemistry,” Natural Product Reports, vol. 19, no. 6, pp. 693–718, 2002.
- V. N. Gladyshev, “Selenoproteins and selenoproteomes,” in Selenium: Its Molecular Biology and Role in Human Health, D. L. Hatfield, M. J. Berry, and V. N. Gladyshev, Eds., pp. 99–114, Springer, New York, NY, USA, 2nd edition, 2006.
- F. Zinoni, A. Birkmann, T. C. Stadtman, and A. Bock, “Nucleotide sequence and expression of the selenocysteine-containing polypeptide of formate dehydrogenase (formate-hydrogen-lyase-linked) from Escherichia coli,” Proceedings of the National Academy of Sciences of the United States of America, vol. 83, no. 13, pp. 4650–4654, 1986.
- F. Zinoni, A. Birkmann, W. Leinfelder, and A. Bock, “Cotranslational insertion of selenocysteine into formate dehydrogenase from Escherichia coli directed by a UGA codon,” Proceedings of the National Academy of Sciences of the United States of America, vol. 84, no. 10, pp. 3156–3160, 1987.
- G. Sawers, J. Heider, E. Zehelein, and A. Bock, “Expression and operon structure of the sel genes of Escherichia coli and identification of a third selenium-containing formate dehydrogenase isoenzyme,” Journal of Bacteriology, vol. 173, no. 16, pp. 4983–4993, 1991.
- W. Leinfelder, K. Forchhammer, F. Zinoni, G. Sawers, M. A. Mandrand-Berthelot, and A. Böck, “Escherichia coli genes whose products are involved in selenium metabolism,” Journal of Bacteriology, vol. 170, no. 2, pp. 540–546, 1988.
- K. Schwarz and C. M. Foltz, “Selenium as an integral part of factor 3 against dietary necrotic liver degeneration,” Journal of the American Chemical Society, vol. 79, no. 12, pp. 3292–3293, 1957.
- M. Vinceti, E. T. Wei, C. Malagoli, M. Bergomi, and G. Vivoli, “Adverse health effects of selenium in humans,” Reviews on Environmental Health, vol. 16, no. 4, pp. 233–251, 2001.
- A. Berken, M. M. Mulholland, D. L. LeDuc, and N. Terry, “Genetic engineering of plants to enhance selenium phytoremediation,” Critical Reviews in Plant Sciences, vol. 21, no. 6, pp. 567–582, 2002.
- G. S. Ahluwalia, Y. R. Saxena, and H. H. Williams, “Quantitative studies on selenite metabolism in Escherichia coli,” Archives of Biochemistry and Biophysics, vol. 124, pp. 79–84, 1968.
- T. L. Gerrard, J. N. Telford, and H. H. Williams, “Detection of selenium deposits in Escherichia coli by electron microscopy,” Journal of Bacteriology, vol. 119, no. 3, pp. 1057–1060, 1974.
- R. J. Turner, J. H. Weiner, and D. E. Taylor, “Selenium metabolism in Escherichia coli,” Biometals, vol. 11, no. 3, pp. 223–227, 1998.
- J. F. Stolz, P. Basu, J. M. Santini, and R. S. Oremland, “Arsenic and selenium in microbial metabolism,” Annual Review of Microbiology, vol. 60, pp. 107–130, 2006.
- J. W. Doran, “Microorganisms and the biological cycling of selenium,” in Advances in Microbial Ecology, K. L. Marshall, Ed., pp. l–32, Plenum Press, New York, NY, USA, 1982.
- C. Garbisu, S. Gonzalez, W.-H. Yang et al., “Physiological mechanisms regulating the conversion of selenite to elemental selenium by Bacillus subtilis,” Biofactors, vol. 5, no. 1, pp. 29–37, 1995.
- A. Yamada, M. Miyashita, K. Inoue, and T. Matsunaga, “Extracellular reduction of selenite by a novel marine photosynthetic bacterium,” Applied Microbiology and Biotechnology, vol. 48, no. 3, pp. 367–372, 1997.
- R. S. Dungan and W. T. Frankenberger Jr., “Reduction of selenite to elemental selenium by Enterobacter cloacae SLD1a-1,” Journal of Environmental Quality, vol. 27, no. 6, pp. 1301–1306, 1998.
- J. Kessi, M. Ramuz, E. Wehrli, M. Spycher, and R. Bachofen, “Reduction of selenite and detoxification of elemental selenium by the phototrophic bacterium Rhodospirillum rubrum,” Applied and Environmental Microbiology, vol. 65, no. 11, pp. 4734–4740, 1999.
- W. J. Hunter and L. D. Kuykendall, “Identification and characterization of an Aeromonas salmonicida (syn Haemophilus piscium) strain that reduces selenite to elemental red selenium,” Current Microbiology, vol. 52, no. 4, pp. 305–309, 2006.
- W. J. Hunter, “An Azospira oryzae (syn Dechlorosoma suillum) strain that reduces selenate and selenite to elemental red selenium,” Current Microbiology, vol. 54, no. 5, pp. 376–381, 2007.
- W. J. Hunter and L. D. Kuykendall, “Reduction of selenite to elemental red selenium by Rhizobium sp. strain B1,” Current Microbiology, vol. 55, no. 4, pp. 344–349, 2007.
- W. J. Hunter, L. D. Kuykendall, and D. K. Manter, “Rhizobium selenireducens sp. nov.: a selenite-reducing α-Proteobacteria isolated from a bioreactor,” Current Microbiology, vol. 55, no. 5, pp. 455–460, 2007.
- W. J. Hunter and D. K. Manter, “Bio-reduction of selenite to elemental red selenium by Tetrathiobacter kashmirensis,” Current Microbiology, vol. 57, no. 1, pp. 83–88, 2008.
- C. I. Pearce, V. S. Coker, J. M. Charnock et al., “Microbial manufacture of chalcogenide-based nanoparticles via the reduction of selenite using Veillonella atypica: an in situ EXAFS study,” Nanotechnology, vol. 19, no. 15, Article ID 155603, 2008.
- W. J. Hunter and D. K. Manter, “Pseudomonas seleniipraecipitatus sp. nov.: a selenite reducing γ-Proteobacteria isolated from Soil,” Current Microbiology, vol. 62, no. 2, pp. 565–569, 2011.
- M. Kabiri, M. A. Amoozegar, M. Tabebordbar, K. Gilany, and G. H. Salekdeh, “Effects of selenite and tellurite on growth, physiology, and proteome of a moderately halophilic bacterium,” Journal of Proteome Research, vol. 8, no. 6, pp. 3098–3108, 2009.
- P. Bao, H. Huang, Z. Y. Hu et al., “Impact of temperature, CO2 fixation and nitrate reduction on selenium reduction, by a paddy soil Clostridium strain,” Journal of Applied Microbiology, vol. 114, no. 3, pp. 703–712, 2013.
- N. Yee, “Geomicrobiology of selenium: life and death by selenite,” Applied Geochemistry, vol. 26, pp. S324–S325, 2011.
- R. S. Dungan, S. R. Yates, and W. T. Frankenberger Jr., “Transformations of selenate and selenite by Stenotrophomonas maltophilia isolated from a seleniferous agricultural drainage pond sediment,” Environmental Microbiology, vol. 5, no. 4, pp. 287–295, 2003.
- M. Bébien, G. Lagniel, J. Garin, D. Touati, A. Verméglio, and J. Labarre, “Involvement of superoxide dismutases in the response of Escherichia coli to selenium oxides,” Journal of Bacteriology, vol. 184, no. 6, pp. 1556–1564, 2002.
- J. Guzzo and M. S. Dubow, “A novel selenite- and tellurite-inducible gene in Escherichia coli,” Applied and Environmental Microbiology, vol. 66, no. 11, pp. 4972–4978, 2000.
- P. Hu, E. L. Brodie, Y. Suzuki, H. H. McAdams, and G. L. Andersen, “Whole-genome transcriptional analysis of heavy metal stresses in Caulobacter crescentus,” Journal of Bacteriology, vol. 187, no. 24, pp. 8437–8449, 2005.
- G. Sawers, “The hydrogenases and formate dehydrogenases of Escherichia coli,” Antonie van Leeuwenhoek, vol. 66, no. 1–3, pp. 57–88, 1994.
- M. D. Wolfe, F. Ahmed, G. M. Lacourciere, C. T. Lauhon, T. C. Stadtman, and T. J. Larson, “Functional diversity of the rhodanese homology domain: the Escherichia coli ybbB gene encodes a selenophosphate-dependent tRNA 2-selenouridine synthase,” Journal of Biological Chemistry, vol. 279, no. 3, pp. 1801–1809, 2004.
- H. Mihara, M. Maeda, T. Fujii, T. Kurihara, Y. Hata, and N. Esaki, “A nifS-like gene, csdB, encodes an Escherichia coli counterpart of mammalian selenocysteine lyase. Gene cloning, purification, characterization and preliminary X-ray crystallographic studies,” Journal of Biological Chemistry, vol. 274, no. 21, pp. 14768–14772, 1999.
- R. Kambampati and C. T. Lauhon, “IscS is a sulfurtransferase for the in vitro biosynthesis of 4- thiouridine in Escherichia coli tRNA,” Biochemistry, vol. 38, no. 50, pp. 16561–16568, 1999.
- A. D. Hollenbach, K. A. Dickson, and M. W. Washabaugh, “Thiamin transport in Escherichia coli: the mechanism of inhibition by the sulfhydryl-specific modifier N-ethylmaleimide,” Biochimica et Biophysica Acta: Biomembranes, vol. 1564, no. 2, pp. 421–428, 2002.
- M. Riley, T. Abe, M. B. Arnaud et al., “Escherichia coli K-12: a cooperatively developed annotation snapshot—2005,” Nucleic Acids Research, vol. 34, no. 1, pp. 1–9, 2006.
- C.-Y. Hung, Y.-H. Sun, J. Chen et al., “Identification of a Mg-protoporphyrin IX monomethyl ester cyclase homologue, EaZIP, differentially expressed in variegated Epipremnum aureum “Golden Pothos” is achieved through a unique method of comparative study using tissue regenerated plants,” Journal of Experimental Botany, vol. 61, no. 5, pp. 1483–1493, 2010.
- F. R. Blattner, G. Plunkett III, C. A. Bloch et al., “The complete genome sequence of Escherichia coli K-12,” Science, vol. 277, no. 5331, pp. 1453–1462, 1997.
- D. B. Cowie and G. N. Cohen, “Biosynthesis by Escherichia coli of active altered proteins containing selenium instead of sulfur,” Biochimica et Biophysica Acta, vol. 26, no. 2, pp. 252–261, 1957.
- T. Tuve and H. H. Williams, “Metabolism of selenium by Escherichia coli: biosynthesis of selenomethionine,” The Journal of Biological Chemistry, vol. 236, pp. 597–601, 1961.
- M. Jormakka, B. Byrne, and S. Iwata, “Formate dehydrogenase—a versatile enzyme in changing environments,” Current Opinion in Structural Biology, vol. 13, no. 4, pp. 418–423, 2003.
- J. C. Boyington, V. N. Gladyshev, S. V. Khangulov, T. C. Stadtman, and P. D. Sun, “Crystal structure of formate dehydrogenase H: catalysis involving Mo, molybdopterin, selenocysteine, and an Fe4S4 cluster,” Science, vol. 275, no. 5304, pp. 1305–1308, 1997.
- W. B. Whitman and C. Jeanthon, “The methanococcales,” in The Prokaryotes, M. Dworkin, S. Falkow, E. Rosenderg et al., Eds., pp. 257–273, Springer, New York, NY, USA, 3rd edition, 2006.
- D. Touati, “Iron and oxidative stress in bacteria,” Archives of Biochemistry and Biophysics, vol. 373, no. 1, pp. 1–6, 2000.
- H. Mihara, S.-I. Kato, G. M. Lacourciere et al., “The iscS gene is essential for the biosynthesis of 2-selenouridine in tRNA and the selenocysteine-containing formate dehydrogenase H,” Proceedings of the National Academy of Sciences of the United States of America, vol. 99, no. 10, pp. 6679–6683, 2002.
- T. Yuen, E. Wurmbach, R. L. Pfeffer, B. J. Ebersole, and S. C. Sealfon, “Accuracy and calibration of commercial oligonucleotide and custom cDNA microarrays,” Nucleic Acids Research, vol. 30, no. 10, article e48, 2002.
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