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Recent studies have demonstrated that photosynthetic cyanobacteria could be an excellent cell factory to produce renewable biofuels and chemicals due to their capability to utilize solar energy and CO2 as the sole energy and carbon sources. Biosynthesis of carbon-neutral biofuel alkanes with good chemical and physical properties has been proposed. However, to make the process economically feasible, one major hurdle to improve the low cell tolerance to alkanes needed to be overcome.
Towards the goal to develop robust and high-alkane-tolerant hosts, in this study, the responses of model cyanobacterial Synechocystis PCC 6803 to hexane, a representative of alkane, were investigated using a quantitative proteomics approach with iTRAQ - LC-MS/MS technologies. In total, 1,492 unique proteins were identified, representing about 42% of all predicted protein in the Synechocystis genome. Among all proteins identified, a total of 164 and 77 proteins were found up- and down-regulated, respectively. Functional annotation and KEGG pathway enrichment analyses showed that common stress responses were induced by hexane in Synechocystis. Notably, a large number of transporters and membrane-bound proteins, proteins against oxidative stress and proteins related to sulfur relay system and photosynthesis were induced, suggesting that they are possibly the major protection mechanisms against hexane toxicity.
The study provided the first comprehensive view of the complicated molecular mechanism employed by cyanobacterial model species, Synechocystis to defend against hexane stress. The study also provided a list of potential targets to engineer Synechocystis against hexane stress.
Human society has been depending on fossil fuels in the past centuries. However, fossil fuels are not infinite resources, and a sharp price increase of these natural resources in recent years has posed an urgent call for alternative ways to produce fuels and chemicals. Moreover, over-utilizing fossil fuels has also caused environmental issues such as global warming and pollution. To address these issues, photosynthetic cyanobacteria have attracted significant attention recently as a cell factory to produce renewable biofuels and chemicals due to their capability to utilize solar energy and CO2 as the sole energy and carbon sources [1-4]. In addition, cyanobacteria have a relatively simple genetic background and are easy for genetic manipulation [5,6]. In recent studies, two approaches have been taken to utilize cyanobacteria for biofuel production: i) to isolate fatty acids from lipid-rich cyanobacterial biomass and then convert them chemically to other products, such as biodiesel [7,8]. However, lipid extraction process from cyanobacteria is very energy-intensive and has been one of the major hurdles for commercial application [9-11]; and ii) to employ genetically manipulated cyanobacteria to produce secretable fuel products directly. So far the second approach has led to successful production of a dozen of fuel products in engineered cyanobacterial systems, including ethanol [12,13], ethylene , isoprene , free fatty acids , fatty alcohols , isobutyraldehyde , 1-butanol [19,20] and hydrogen [21,22]. Although the current productivity level by these systems is still very low, the studies clearly demonstrated the feasibility of developing sustainable production systems based on cyanobacterial cells.
Biofuels offer a diverse range of promising alternatives. Although currently ethanol constitutes 90% of all biofuels in the United States, other fuels with better chemical properties, such as bio-based alkane due to their low water solubility and high energy density , are also being pursued around the world [24,25]. Alkanes composed of 5 to 9 carbons, which are liquid at room temperature and among the usual suspects in gasoline, can be used as a good fuel in internal combustion engine , while C8–C21 alkanes are the predominant components of diesel fuel . Biosynthesis of alkanes has also been reported in a diversity of microorganisms including photosynthetic cyanobacteria since later 1960s [24,27,28]; however, its production in native producing hosts has not received much attention due to their low productivity. In a recent study, the researchers isolated a biosynthesis pathway consisting of an acyl-acyl carrier protein reductase and an aldehyde decarbonylase, which together convert intermediates of fatty acid metabolism to alkanes and alkenes in cyanobacterium Synechococcus elongatus, and expressed it heterologously in Escherichia coli, leading to the production and secretion of C13 to C17 mixtures of alkanes at~0.3g/L after 40h cultivation in E. coli. The work for the first time demonstrated the potential to use heterologous hosts for high–efficiency alkane production. Currently efforts are ongoing in both academic and industry settings to express synthetic alkane pathways in photosynthetic cyanobacterial hosts for the production of the third-generation carbon-neutral biofuels.
As solvents, alkane products are toxic to microbes . Their toxicity is inversely correlated with the logPow value, which is the common logarithm of the partition coefficient (Pow) for the distribution of the organic solvent between n-octanol and water phases [31,32]. A series of genes involved in alkane tolerance in E. coli have been identified and utilized as targets to improve alkane tolerance by genetic engineering, which has led to some progress in improving alkane tolerance in E. coli[33-37]. Cyanobacteria have low tolerance to alkanes; meanwhile, currently the knowledge on alkane tolerance in cyanobacteria is very limiting. To fully understand the effects of alkane on the cyanobacterial cells so that a construction of more robust alkane-producing cyanobacterial hosts can be possible, in this study, we employed a quantitative proteomics approach with isobaric tag for relative and absolute quantification (iTRAQ) technique and liquid chromatography-tandem mass spectrometry (LC-MS/MS) to reveal the global metabolic response of the model cyanobacterium Synechocystis to the treatment of hexane, a representative alkane. The results showed that common stress responses which have been reported for other microbes under solvent/biofuel stress were induced by hexane in Synechocystis. Notably, the analysis revealed the induction of large numbers of transporters and membrane-bound proteins, proteins related to sulfur relay system, oxidative stress response and photosynthesis, suggesting that they were among the major protection mechanisms against hexane. The study provided the first comprehensive view of the complicated molecular mechanism employed by cyanobacterial model species, Synechocystis to defend against hexane stress, and also constituted an important foundation for rational engineering of more robust photosynthetic hosts for the production of the carbon-neutral biofuel alkane.
The growth of Synechocystis supplemented with 0, 0.7%, 0.8% and 0.9% hexane was assessed to determine an appropriate hexane concentration for proteomic studies (Figure (Figure1).1). The results showed that the hexane concentration that caused an approximately 50% growth inhibition was found to be 0.8% (v/v) at both 24h and 48h (corresponding to middle-exponential and exponential-stationary transition phases, respectively), and was selected for the proteomics analysis in this study. The tolerance level of Synechocystis to hexane was similar to what has been reported for Aeromonas hydrophila and Pseudomonas aeruginosa. Cell morphology examination showed no visible change after hexane treatment (data not shown). For proteomic analysis, two independent cultivations for both control and 0.8% hexane treatment were conducted, and cells were collected by centrifugation (8,000 x g for 10min at 4°C) at 24h and 48h, resulting in two biological replicates for each time point of control and hexane-treated samples (Figure (Figure1).1).
A total of 167,191 spectra were obtained from the iTRAQ - LC-MS/MS proteomic analysis. After data filtering to eliminate low-scoring spectra, a total of 24,162 unique spectra that met the strict confidence criteria for identification were matched to 1,491 unique proteins, representing approximately 41.8% of the 3569 predicted proteins in the Synechocystis genome ( Additional file 1: Table S1). In terms of protein molecular weight (MW) distribution, good coverage (averages of 30–45% of the total proteins in each MW group) was obtained for a wide MW range for proteins larger than 10kDa (Figure (Figure2A).2A). In addition, most of the proteins were identified with good peptide coverage, of which ~65% of the proteins were with more than 10% of the sequence coverage, and ~44% were with 20% of the sequence coverage (Figure (Figure2B).2B). Among all the proteins detected, 1,181 and 1,172 were identified from the samples of 24h and 48h, respectively. The proteins that were identified only in control or treated samples so that ratio calculation is not available were excluded from the analysis. Based on the number of unique proteins identified in each functional category, the most frequently detected functional categories were “general function prediction only” and “signal transduction mechanisms”, representing 11.1% and 10.85% of all the protein identified, respectively (Figure (Figure2C).2C). Proteins involved in signal transduction network are generally with low abundance, quick protein turnover time and membrane-bound , a high coverage of the group of signal proteins also suggested the methodology used in the study is with high sensitivity and very reliable. The high percentage of functionally unknown proteins identified is not unreasonable, considering more than 40% of proteins in the Synechocystis genome are still annotated as hypothetical proteins without any functional prediction. Other most frequently detected functional categories included “amino acid transportation and metabolism” (9.17%), “energy production and conversion” (7.55%), and “translation, ribosomal structure and biogenesis” (7.55%) and “cell wall/membrane/envelope biogenesis” (7.24%), suggested that the proteins in these functional categories were highly expressed and may be active during the growth and treatment conditions.
Reproducibility of the proteomic analysis was assessed in two types of comparisons (Figure (Figure3).3). First we labeled and mixed two biological replicates of a given condition directly for proteomic analysis (i.e. biological replicate 1 and 2 of control at 24h, replicate 1 and 2 of control at 48h, biological replicate 1 and 2 of hexane treatment at 24h, biological replicate 1 and 2 of hexane treatment at 48h), the difference was plotted verse the percentage of the proteins identified, the results showed that approximately 60% of the proteins with difference less than delta error of 0.1, and more than 95% of the proteins with difference less than delta error of 0.5 (Figure (Figure3-I).3-I). Second we labeled and mixed each pair of hexane-treated sample and its control for proteomic analysis, the difference between different biological pairs was plotted in Figure Figure3-II.3-II. The dispersion of the iTRAQ ratios of the quantified proteins (i.e. 1,181 and 1,172 for 24h and 48h, respectively) was found with very similar trends between four biological replicates at either 24h (Figure (Figure3-II-A)3-II-A) or 48h (Figure (Figure3-II-B),3-II-B), suggesting that the biological noise was reasonably low.
Using a cutoff of 1.5-fold change and a p-value less than 0.05, we determined that 140 and 148 unique proteins were differentially regulated between control and hexane treatments conditions at 24h and 48h, respectively ( Additional file 1: Table S1). Among them, a total of 164 and 77 proteins were up-regulated and down-regulated by the hexane treatments, respectively. Forty-two up-regulated and 4 down-regulated proteins were shared between 24h and 48h, while more of the responsive proteins were unique for each of the time points, consistent with the expected physiological differences between middle-exponential and transition phases of the cell growth (Figure (Figure11).
Metabolic pathway enrichment analysis was carried out for the differentially regulated proteins to determine the affected cellular metabolism ( Additional file 2: Table S2). The analysis was performed by matching the responsive proteins to the proteins annotated with KEGG Pathway database, and then comparing the frequencies of the responsive proteins in each KEGG pathway to determine statistically authenticity of the involvement of that KEGG pathway in hexane response. A series of KEGG pathways affected by the hexane treatment, with p-value less than 0.05 as cut off were identified. The results showed that at 24h after hexane treatment, four KEGG pathways were differentially regulated by the hexane treatment: they are “Ribosome” (KO03010), “Sulfur relay system” (KO04122), “Photosynthesis” (KO00195) and “Arachidonic acid metabolism” (KO00590). All four pathways were enriched by at least two out of four biological replicates, with “Ribosome” (KO03010) enriched with good confidence in all four replicates and “Photosynthesis” (KO00195) enriched in two replicates, consistent with the relatively high expression of ribosomal proteins and photosynthetic proteins, and the sensitivity of protein biosynthesis and photosynthetic processes to stress. Most of the ribosomal proteins identified were down-regulated, suggesting an overall slowdown of the protein biosynthesis and possible slow metabolism. At 48h, five KGG pathways, “Sulfur relay system” (KO04122), “ABC transporters” (KO02010), “Photosynthesis” (KO00195), “Steroid biosynthesis” (KO00100), and “Biosynthesis of ansamycins” (KO01051) were enriched by the differentially expressed proteins. Although these KEGG pathways were enriched in only two out of four biological replicates, the p-values were reasonably low, suggesting in general the reliability of the data analysis. The enrichment of “Ribosome” pathway (KO03010) at only 24h was interesting, which may implicate that modification of the primary metabolism, such as protein biosynthesis, may be one of the major strategies that cells used to deal with stress during middle-exponential phase. In this study, we found that several ribosomal proteins, Sll1816 (rpsM), Sll1803 (rplV) and Ssr0482 (rpsP) were down-regulated under hexane treatment. Interestingly, these three genes, rpsM, rplV, and rpsP, were named as targets as they were also down-regulated in E. coli against organic solvent also indicated .
“Sulfur relay system” (KO04122) was differentially regulated at both 24 and 48h, in three out of four biological replicates at 24h, and two out of four biological replicates at 48h, respectively ( Additional file 2: Table S2). The sulfur-relay system classified in tRNA modification has been demonstrated to modify a few nucleotides of tRNA molecules, their increased expression has been reported contributing to stabilization of their structure, and was required for survival at an extremely high temperature in E. coli and Thermous thermophilus. In addition, ubiquitin (Ub) like proteins are signaling messengers that control many cellular functions in bacteria. It has been proposed that the Ub-protein modification evolved from prokaryotic sulfurtransfer systems . Molybdenum cofactor (Moco) and thiamin are sulfur-containing cofactors whose biosynthesis includes a key sulfur transfer step that uses unique sulfur carrier proteins, MoaD and ThiS. Detailed analysis showed that upon hexane stress, two proteins in “Sulfur relay system” pathway, Slr0821 and Ssl1707 with homologies to sulfur carrier proteins MoaD and sulfur-accepting protein TusA were up-regulated, consistent with their possible roles against stress.
As one core function of cyanobacteria, “Photosynthesis” pathway (KO00195) was differentially regulated by hexane exposure at both 24h and 48h, in two out of four biological replicates ( Additional file 2: Table S2). Early studies showed that some natural stresses, such as salt and sulfur starvation, decreased expression level of genes for phycobilisome, photosystems I and II, cytochrome b6/f, and ATP synthase, indicating overall reduced light-harvesting and photosynthetic activity upon stress [43,44]. However, detailed analysis showed that six proteins involved in photosystem I and II (Slr0172: photosystem I assembly protein; Sll0629: photosystem I subunit X; Slr1645: photosystem II 11 kD protein; Sll1194: photosystem II complex extrinsic protein precursor U; Sll1418: photosystem II oxygen-evolving complex 23K protein PsbP homolog; and Sll1398: photosystem II reaction center protein Psb28), four ferredoxin proteins (Slr1828, Ssl0020, Sll1382, Slr1205) and two cytochrome (Ssr3451: cytochrome B559 subunit alpha; and Sll0258: cytochrome C-550) were all up-regulated by hexane exposure (Table (Table1).1). Although it remains unclear how the increased expression of photosynthesis-related proteins will help combat the hexane toxicity, the results were consistent with our recent study on ethanol toxicity in Synechocystis sp. PCC 6803, where the similar proteomics analysis also demonstrated a profoundly increased expression of many proteins related to photosynthesis .
“Arachidonic acid metabolism” pathway (KO00590) was differentially regulated by hexane exposure at 24h, in two out of four biological replicates ( Additional file 2: Table S2). Detailed analysis showed two proteins of glutathione peroxidase (Slr1992 and Slr1171) were up-regulated and thus contributed to the enrichment of this pathway (Table (Table1).1). Peroxidases are heme-cofactored enzymes responsible for hydrogen peroxide removal, cytoplasmic glutathione peroxidase (Gpx) has been found involved in oxidative defense in many bacteria .
“Steroid biosynthesis” pathway (KO00100) was differentially regulated by hexane exposure at 48h ( Additional file 2: Table S2). Detailed analysis showed that sll0513 encoding a putative squalene synthase was down-regulated, which then contributed to the enrichment of this pathway (Table (Table2).2). Role of this enzyme in cyanobacteria upon hexane stress still needs more investigation, but it has been reported that squalene synthase (Erg9) in yeast was down regulated upon oxidative stress and ergosterol level plays a key role in adaptation to oxidative stress .
Pathway enrichment analysis showed that “ABC transporters” (KO02010) was differentially regulated by hexane exposure, among which four ABC transporters were matched to the KEGG pathway KO02010 at 48h ( Additional file 2: Table S2). Further analysis, however, showed that more putative transporters were up-regulated by the hexane treatment (Table (Table1).1). Induction of transporters by stress or toxic solvent has been reported in many microbes, such as acrAB-tolC in E. coli and srpABC in Pseudomonas putida which have been shown to export hexane, heptane, octane, octanol and nonane, and the enhanced expression of these genes were related to high tolerance [48,49]. Up-regulation of transporters has been reported for various stresses in many other cyanobacterial species, such as arsenate resistance in Anabaena variabilis, salinity in Synechocystis[50-53]. In Synechocystis sp. PCC 6803, we recently found that five putative transporters involved in transporting of different substrates (i.e. polar amino acid, bicarbonate, iron, Na+/K+) were up-regulated by ethanol exposure . Upon hexane exposure, a spectrum of putative transporters, including five transporters involved in bicarbonate transporting (Slr0041, Slr0043, Sll0834, Slr1512, Sll1734), two involved in cation transporting (Slr2131, Sll0672), two involved in Na+ and K+ transporting (Sll0689, Sll0493), one involved in mercuric transporting (Ssr2857), were up-regulated (Table (Table1).1). In Synechocystis sp. PCC 6803, the slr0040, slr0041, slr0043, and slr0044 genes, forming an operon with a putative porin gene (slr0042), were induced under low CO2 stress conditions to increase the bicarbonate transporting . Slr1512 was previously found essential to Na+-dependent HCO3- transport and may play a crucial role in carbon acquisition when CO2 supply is limited . sll0493 encodes an NAD+-binding peripheral membrane protein (KtrA) that by working with a K+ transporters (KtrB; Slr1509) and KtrE (Slr1508), played a crucial role in the early phase of cell turgor regulation after hyperosmotic shock in Synechocystis. Although the preliminary evidence suggested that these transporters may directly involve in hexane transporting, their up-regulation implicated the important roles for the hexane tolerance.
In addition, our proteomic analysis showed that many proteins located on cell membrane were up-regulated (Table (Table1),1), including a plasma membrane protein essential for thylakoid formation Sll0617 (vipp1) with a similar gene, pspA, in E. coli up-regulated by organic solvents , a periplasmic iron-binding protein (Slr0513) , four periplasmic proteins with unknown function (Slr1160, Slr2144, Slr1513, Sll0319), a salt-enhanced periplasmic protein (Sll1549). Meanwhile, several membrane-bound proteins were also found down-regulated by hexane exposure (Table (Table2).2). Although the exact function of these proteins was mostly unknown, the significant changes occurred at the cell membrane level may represent an important resistance strategy against hexane toxicity.
Bacteria use a variety of secretion systems to transport proteins beyond their cell membrane in order to interact with their environment. In E. coli and other gram-negative bacteria, one of the major translocation systems is the twin arginine translocation pathway consisted of TatA, TatB and TatC to export folded proteins across the cytoplasmic membrane ; and another is the Sec-dependent protein translocation system whose complex molecular machine comprises a flexible transmembrane conduit coupled to a motor-like component . Our proteomics analysis showed that hexane treatment induced the expression of both systems in Synechocystis sp. PCC 6803. The putative TatA protein (Slr1046) of twin arginine translocation pathway and SecF (Slr0775) of the Sec-dependent protein translocation system were both up-regulated (Table (Table11).
Two-component system (TCS) is an important signal transduction mechanism employed by prokaryotes to survive the complex and volatile environments , and has been involved in various stress responses in cyanobacteria [61,62]. In our previous work, two response regulators (Slr1783, Slr1909) were found up-regulated by ethanol exposure; however, these two response regulators were not differentially regulated by hexane under our experimental conditions ; meanwhile, four different regulatory proteins were up-regulated, and two regulatory proteins were down-regulated by hexane exposure (Table (Table1,1, ,2).2). Interestingly, up-regulated Slr1697 of a serine/threonine kinase and up-regulated Sll0043 of a positive phototaxis hybrid histidine kinase (homologous to chemotaxis protein CheA) were both required for cell motility and chemotaxis [63,64]. Chemotaxis and flagellar motility are essential mechanisms by which bacteria use to adapt to and survive in environments suffered with various natural stresses , our results showed that the Synechocystis cells may adapt the similar mechanism in dealing with the stress caused by hexane. In addition, the fact that a different set of regulatory proteins were involved in hexane stress from those in ethanol stress implicated that variable resistance mechanisms were used by the cells for the biofuel products of different chemical properties .
Early studies have defined a set of common stress responses that cells will typically initiate upon stresses from organic solvent or biofuel products, including down-regulation of ribosomal proteins, induction of heat shock proteins to aid with proper protein folding, induction of oxidative stress response, and modification of cell membrane [66-68]. Our proteomic analysis showed that the initiation of these common stress response programs were also seen in the hexane-treated Synechocystis cells, although the protein species used for each of the function could vary between microbial species (Table (Table1,1, ,2).2). For example, a heat shock protein (GrpE, Sll0057) was induced by hexane in the Synechocystis cells, while in E. coli treated with one of the hydrophobic organic solvents, n-hexane or cyclooctane, a 28kDa phage-shock protein PspA was induced . While in the ethanol-treated Synechocystis cells, two heat shock proteins, GroES (Slr2075) and GrpE (Sll0057) were up-regulated . Oxidative stress responses have been reported for cells under treatment of organic solvents as they induced production of highly reactive oxygen species (ROS). Without exception, ROS formation has been suggested playing a important role in n-hexane induced alterations in cell proliferation and membrane integrity . In addition to two responsive glutathione peroxidase discussed above, our proteomic analysis showed that a bacterioferritin comigratory protein (Slr0242), a rehydrin (Slr1198) and a methionine sulfoxide reductase A (Sll1394) were also induced in response to the oxidative stress caused by hexane in Synechocystis (Table (Table1).1). Studies of solvent-tolerant microbes found that cells can modify fatty acid composition or other accessory molecules of their cell membrane to block the entry of solvents [66,67]. Up-regulation of Slr1761, a peptidylprolyl cistrans isomerase which catalyses the cistrans isomerization of proline imidic peptide bonds in oligopeptides in both prokaryotic and eukaryotic cell envelope upon stress, was found in hexane-treated cells, similar up-regulation of Slr1761 by ethanol was also observed previously Synechocystis.
Alkane compounds of varying carbon lengths have been proposed as a good alternative to gasoline. However, one of the major hurdles needed to be overcome is that alkanes typically exhibit toxicity to microbes, especially cyanobacterial cells. Towards this end, we employed a global-based quantitative proteomics approach with iTRAQ - LC-MS/MS technologies to reveal the responses of Synechocystis to hexane, a representative of alkane. Using a cutoff of 1.5-fold change and a p-value less than 0.05, a total of 164 up-regulated and 77 down-regulated proteins were determined. Function annotation and KEGG pathway enrichment analyses showed that common stress responses which have been reported for other microbes under organic solvent/biofuel stress were also induced in Synechocystis[66,67]. Notably, the analysis revealed the induction of a large number of transporters and membrane-bound proteins, proteins related to sulfur relay system, oxidative stress and photosynthesis, suggesting that they were among the major protection mechanisms against hexane. In this study hexane is added exogenously, however, it is expected that the general responses uncovered by the study will be similar to that caused by hexane generated intracellularly, although intracellular hexane may be more toxic at lower concentration. Nevertheless, the study provided the first comprehensive view of the complicated molecular mechanism employed by cyanobacterial model species, Synechocystis to defend against hexane stress. Moreover, the proteomic analysis identified a list of potential target genes/proteins which can be engineered to generate stress-resistant hosts for high efficiency production of hexane [71,72].
Synechocystis sp. PCC 6803 was obtained from American Type Culture Collection (ATCC) and grown in BG11 medium (pH 7.5) under a light intensity of approximately 50μmol photons m-2s-1 in an illuminating incubator operated at 130rpm and at 30°C (HNY-211B Illuminating Shaker, Honour, China) [73-75]. Cell density was measured on a UV-1750 spectrophotometer (Shimadzu, Japan). For growth and hexane treatment, the 10mL fresh cells of OD730 0.5 were collected by centrifugation at 8000 x g for 10min at 4°C, and then were inoculated into 50mL BG11 liquid medium in a 250-mL flask. Hexane of varying concentration was added at the beginning of cultivation. 1mL of culture samples were collected and measured with a spectrophotometer at OD730 every 12h. Morphology of Synechocystis under control and treatment conditions was observed using a BX43 fluorescence microscope (Olympus, Japan). Growth experiments were repeated at least three times to confirm the growth patterns. Cells for proteomics analysis were collected by centrifugation at 8,000 x g for 10min at 4°C.
For each sample, 10mg of cells were frozen by liquid nitrogen immediately after centrifugation and washed with phosphate buffer (pH 7.2). The cells were broken with sonication cracking at low temperature. Cell pellets were then resuspended in a lysis buffer (8M urea, 4% CHAPS, 40mM Tris–HCl), with 1mM PMSF and 2mM Ethylenediaminetetraacetic acid (EDTA) (final concentration). After 5min of vigorously vortex, dithiothreitol (DTT) was also added to a final concentration of 10mM. After mix, the sample were centrifuged for 20min at 20,000 x g, and the supernatant was mixed well with ice-cold acetone (1:4, v/v) with 30mM DTT. After repeating this step twice, supernatants were combined and precipitated at −20°C overnight, and stored at −80°C prior to sample if not for immediate use. For digestion, protein pellet from previous step was resuspended in digestion buffer (100mM triethylammonium bicarbonate TEAB, 0.05%w/v sodium dodecyl sulfate, SDS) to a final concentration of 1mg/mL (total protein measured by bicinchonic acid assay (Sigma, St. Louis, MO)). Equal aliquots (500μg) from each lysate were then digested with trypsin overnight at 37°C (Sigma; 1:40 w/w added at 0 and 2h) and lyophilized.
The iTRAQ labeling of peptide samples derived from control and hexane treatment conditions were performed using iTRAQ reagent Multiplex kit (Applied Biosystems, Foster City, CA) according to manufacturer’s protocol. For each time point (i.e. 24h or 48h), four samples (two biological replicates for control and two biological replicates for hexane-treated samples) were iTRAQ labeled. The peptides labeled with respective isobaric tags, incubated for 2h and vacuum centrifuged to dryness. The labeled control and hexane treatment replicate samples were 1:1 pooled, and generating four combinations of samples for each time point, which were reconstituted in Buffer A (10mM KH2PO4, 25% acetonitrile, pH 2.85). The iTRAQ labeled peptides were fractionated using PolySULFOETHYL ATM SCX column (200 x 4.6mm, 5μm particle size, 200 A° pore size) by HPLC system (Shimadzu, Japan) at flow rate 1.0mlmin-1. The 50min HPLC gradient consisted of 100% buffer A (10mM KH2PO4, 25% acetonitrile, pH 2.85) for 5min; 0-20% buffer B (10mM KH2PO4, 25% ACN, 500mM KCL, pH 3.0) for 15min; 20-40% buffer B for 10min; 40-100% buffer B for 5min followed by 100% buffer A for 10min. The chromatograms were recorded at 218nm. The collected fractions were desalted with Sep-Pak® Vac C18 cartridges (Waters, Milford, Massachusetts), concentrated to dryness using vacuum centrifuge and reconstituted in 0.1% formic acid for LC-MS/MS analysis.
The mass spectroscopy analysis was performed using a AB SCIEX TripleTOF™ 5600 mass spectrometer (AB SCIEX, Framingham, MA, USA), coupled with online micro flow HPLC system (Shimadzu, JAPAN) as described before [76,77]. The peptides were separated using nanobored C18 column with a picofrit nanospray tip (75μm ID x 15cm, 5μm particles) (New Objectives, Wubrun, MA). The separation was performed at a constant flow rate of 20μlmin-1, with a splitter to get an effective flow rate of 0.2μlmin-1. The mass spectrometer data acquired in the positive ion mode, with a selected mass range of 300–2000m/z. Peptides with +2 to +4 charge states were selected for MS/MS. The three most abundant peptides above a 5 count threshold were selected for MS/MS and dynamically excluded for 30s with ±30 mDa mass tolerance. Smart information-dependent acquisition (IDA) was activated with automatic collision energy and automatic MS/MS accumulation. The fragment intensity multiplier was set to 20 and maximum accumulation time was 2s. The peak areas of the iTRAQ reporter ions reflect the relative abundance of the proteins in the samples.
The data acquisition was performed with Analyst QS 2.0 software (Applied Biosystems/MDS SCIEX). Protein identification and quantification were performed using Mascot 2.3.02 (Matrix Science, London, United Kingdom) . For iTRAQ quantification, the peptide for quantification was automatically selected by the algorithm to calculate the reporter peak area, error factor (EF) and p-value. The resulting data set was auto bias-corrected to get rid of any variations imparted due to the unequal mixing during combining different labeled samples. Genome sequence and annotation information of Synechocystis were downloaded from NCBI and the Comprehensive Microbial Resource (CMR) of TIGR (http://www.tigr.org/CMR) (April 22, 2012) . Proteins with 1.5 fold change between hexane-treated and control samples and p-value of statistical evaluation less than 0.05 were determined as differentially abundant proteins. Metabolic pathway enrichment analysis of the responsive proteins was conducted according to the information from the KEGG Pathway Database using the following formula:
where N is the number of all proteins with KEGG pathway annotation information, n is the number of the differentially regulated proteins with KEGG pathway annotation information, M is the number of proteins with a given KEGG pathway annotation, m is the number of the differentially regulated proteins with a given KEGG pathway annotation. The KEGG pathways with p-value less than 0.05 were considered as enriched KEGG pathways by the hexane responsive proteins.
iTRAQ: Isobaric tag for relative and absolute quantitation; LC-MS/MS: Liquid chromatography-tandem mass spectrometry; KEGG: Kyoto Encyclopedia of Genes and Genomes; TCS: Two-component system.
The authors declare that they have no competing interests.
LC, JW, and WZ conceived of the study. LC, LW, JL, JQ and WZ drafted the manuscript. JL, LC, JW, and WZ carried out cultivation, protein isolation and proteomics analysis. LC, JW and WZ finish the statistical analysis for proteomics data. “All authors read and approved the final manuscript.”
Table S1. Full list of identified proteins and their ratio across conditions *.
Table S2. KEGG pathway enrichment analysis of the differentially regulated proteins *.
The research was supported by grants from National Basic Research Program of China (National “973” program, project No. 2011CBA00803 and No. 2012CB721101). The authors would also like to thank Tianjin University and the “985 Project” of Ministry of Education for their generous supports in establishing the research laboratory.