physiology and proteomics of the water-deficit stress...
TRANSCRIPT
Physiology and proteomics of the water-deficit stressresponse in three contrasting peanut genotypes
KAMESWARA RAO KOTTAPALLI1,2, RANDEEP RAKWAL3,4, JUNKO SHIBATO3, GLORIA BUROW2,DAVID TISSUE5,6, JOHN BURKE2, NAVEEN PUPPALA7, MARK BUROW1,8 & PAXTON PAYTON2
Departments of 1Plant and Soil Science and 5Biology, Texas Tech University, Lubbock, TX 79409, USA, 2United StatesDepartment of Agriculture Cropping Systems Research Laboratory, Lubbock, TX 79415, USA, 3Health Technology ResearchCenter (HTRC), National Institute of Advanced Industrial Science and Technology WEST, Onogawa 16-1, Tsukuba,305-8569, Japan, 4Research Laboratory for Biotechnology and Biochemistry (RLABB), Kathmandu, Nepal, 6University ofWestern Sydney, Centre for Plant and Food Science, Richmond, NSW 2753, Australia, 7New Mexico State UniversityAgricultural Science Center, Clovis, NM 88101, USA and 8Texas Agrilife Research and Extension Center Texas A&M System,Lubbock, TX 79403, USA
ABSTRACT
Peanut genotypes from the US mini-core collection wereanalysed for changes in leaf proteins during reproductivestage growth under water-deficit stress. One- and two-dimensional gel electrophoresis (1- and 2-DGE) was per-formed on soluble protein extracts of selected tolerantand susceptible genotypes. A total of 102 protein bands/spots were analysed by matrix-assisted laser desorption/ionization–time-of-flight mass spectrometry (MALDI–TOF MS) and by quadrupole time-of-flight tandem massspectrometry (Q-TOF MS/MS) analysis. Forty-nine non-redundant proteins were identified, implicating a variety ofstress response mechanisms in peanut. Lipoxygenase and1L-myo-inositol-1-phosphate synthase, which aid in inter-and intracellular stress signalling, were more abundant intolerant genotypes under water-deficit stress. Acetyl-CoAcarboxylase, a key enzyme of lipid biosynthesis, increased inrelative abundance along with a corresponding increase inepicuticular wax content in the tolerant genotype, suggest-ing an additional mechanism for water conservation andstress tolerance. Additionally, there was a marked decreasein the abundance of several photosynthetic proteins in thetolerant genotype, along with a concomitant decrease innet photosynthesis in response to water-deficit stress. Dif-ferential regulation of leaf proteins involved in a variety ofcellular functions (e.g. cell wall strengthening, signal trans-duction, energy metabolism, cellular detoxification andgene regulation) indicates that these molecules could affectthe molecular mechanism of water-deficit stress tolerancein peanut.
Key-words: 1-DGE; 2-DGE; peanut mini-core; drought.
INTRODUCTION
Legumes are the second most important source of foodin the world (FAOSTAT data 2007), and production ofpeanuts (Arachis hypogaea L.) is second only to soybean,with a total global harvests of 34 million tons (FAOSTATdata 2007). The USA produces nearly two million tons ofpeanuts with an annual worth of $1 billion to farmers and$6 billion to the economy overall (United States Depart-ment of Agriculture Data and Statistics 2006). The majorityof peanut acreage in the south-western USA is in semi-aridregions with limited potential for irrigation, whereas in thesouth-eastern USA approximately half of the peanutacreage is grown under rain-fed conditions. While peanutsare moderately adaptive to water-deficit conditions,increased urban water usage, prolonged drought in thesouthern USA and limited water resources (e.g. rapidlydeclining water table in Ogallala Aquifer) are threateningsustainable peanut crop production. Reductions in watersupply generate water-deficit stress in peanuts and subse-quent loss of yield. Annually, US crop losses caused bydrought exceed $500 million, and it is estimated thatapproximately half of that loss could be avoided by geneticimprovement for water-deficit stress tolerance (Devaiahet al. 2007).
Despite the agronomic and economic impacts of drought,little is known about the molecular mechanisms regulatingwater stress tolerance in peanuts (Jain, Basha & Holbrook2001; Luo et al. 2005). Our knowledge of the molecularresponses to abiotic stress is limited primarily to those asso-ciated with changes in transcription (Seki et al. 2001; Bray2002; Drame et al. 2007). Candidate genes identified duringwater stress include transcriptional regulators, signal trans-duction molecules and genes that protect cells against stress(Seki et al. 2001). Two signalling molecules, a serine-richprotein and a leucine-rich protein, were identified in a waterstress-tolerant peanut (Devaiah et al. 2007). Recently, it wasshown that increased accumulation of phospholipase Daand late embryogenesis abundance (LEA) transcripts mayreduce water loss and protect cellular components against
Correspondence: P. Payton. Fax: +1 806 723 5272; e-mail: [email protected]
Mention of trademark or proprietary product does not constitute aguarantee or warranty of a product by the United States Depart-ment of Agriculture (USDA) and does not imply its approval to theexclusion of other products that may also be suitable.
Plant, Cell and Environment (2009) 32, 380–407 doi: 10.1111/j.1365-3040.2009.01933.x
© 2009 Blackwell Publishing Ltd380
stress damage (Drame et al. 2007). These researchers alsoreported that decreased serine protease expression coulddelay water stress-induced senescence. However, cellularprocesses are also regulated by protein–protein interac-tions, post-translational protein modifications and enzy-matic activities that cannot be identified by gene expressionstudies alone.
Proteomic analyses may, therefore, provide a powerfultool to address biochemical and physiological aspects ofplant response to water-deficit conditions. For example,Bhushan et al. (2007) identified over 100 proteins impli-cated in cell wall modification, signal transduction, metabo-lism and cell defence in the cell wall and extracellularmatrix in chickpea exposed to dehydration stress. Evalua-tion of the mitochondrial proteome in pea indicated thebroader induction of defence strategies and less proteindamage during exposure to water-deficit stress comparedto chilling (Taylor et al. 2005). At the whole cell level, Haj-heidari et al. (2005) identified several key photosyntheticenzymes, including ribulose 1·5-bisphosphate carboxylase/oxygenase (Rubisco), as well as proteins involved in redoxregulation, reactive oxygen scavenging, signal transductionand chaperone activity that were responsive to water-deficitstress in sugar beet leaves. In rice leaves, proteomics analy-sis revealed increased actin depolymerizing factor, anS-like RNase homolog, and Rubisco activase, and down-regulation of isoflavone reductase-like proteins duringwater stress (Salekdeh et al. 2002).
Phenotypic screens of core or mini-core peanut germ-plasm collections have identified variability in many traits,including resistance to both abiotic and biotic stress factors,and aflatoxin contamination (Isleib et al. 1995; Anderson,Holbrook & Culbreath 1996; Holbrook, Wilson &Matheron 1998; Holbrook, Stephenson & Johnson 2000).Variability in plant traits associated with water-deficit stresstolerance has been identified in the ICRISAT mini-corecollection (Upadhyaya 2005), but little is known aboutthese traits in the US germplasm. In most cases, physiologi-cal traits were not examined, and only a few morphologicaltraits (e.g. root length and final yield) were used to assessstress tolerance (Branch & Kvien 1992; Rucker et al. 1995;Holbrook et al. 2000). While this approach has occasionallybeen successful (e.g. C76-16 breeding line; Holbrook et al.2007), initial screens utilizing a primarily yield-based analy-sis for selection of stress tolerance will reject germplasmthat exhibits relatively poor yield under well-watered con-ditions, but has significant potential for tolerance to waterdeficit. Therefore, strategies that employ a greater range offactors are more likely to successfully identify tolerant lines.
Bennett et al. (2002) demonstrated that an integratedapproach to selection for abiotic stress tolerance combin-ing physiological, transcript and protein expression couldreveal differences that were not identified using a singlemethod. For example, in sorghum an integrated approachindicated that aluminium tolerance was controlled by asingle major gene plus several minor genes (Magalhaes2006). Although the complex tolerance mechanisms forstresses like heat and water deficit are not likely to be as
conclusively resolved, identification of key genes, proteinsand physiological responses to these stresses in a large anddiverse set of germplasm will substantially improve ourability to select stress-tolerant plants.
In this study, our objectives were to increase our under-standing of the molecular mechanisms conferringwater-deficit stress tolerance in peanuts and to identifystress-tolerant genotypes. Seventy uniform US mini-coregenotypes and seven peanut cultivars were screened forstress tolerance, and 20 genotypes were selected for addi-tional water-deficit stress screening and physiological analy-ses. We utilized a variety of morphological, physiologicaland proteomic techniques to examine peanut response towell-watered and water-deficit conditions in an environ-mentally controlled glasshouse. Key enzymes and structuralproteins that may be associated with water-deficit stresstolerance were then identified. These results allow us toassociate physiologically significant candidate proteins withwater-deficit stress tolerance mechanism in peanuts.
MATERIALS AND METHODS
Seed material and water-deficitstress treatment
We investigated 70 peanut genotypes from a US peanutmini-core collection (Kottapalli et al. 2007a) and sevenadditional cultivars. After initial screening, 20 genotypes,consisting of 17 mini-core genotypes and three check culti-vars (Table 1), were selected for further evaluation of waterstress tolerance utilizing a chlorophyll fluorescence assay(Burke 2007). Plants were grown from seed in 2 L pots in aglasshouse maintained at an optimal growing temperature(31/27 °C day/night cycle) and natural light conditions;
Table 1. Selected US mini-core genotypes and check cultivarsfor water-deficit stress screening
Mini-core ID PI # Subspecies Market type
COC038 493581 fastigiata ValeniciaCOC041 493631 fastigiata ValeniciaCOC050 493717 fastigiata ValeniciaCOC068 493880 fastigiata ValeniciaCOC149 502040 fastigiata SpanishCOC166 494795 hypogaea RunnerCOC208 274193 hypogaea VirginiaCOC227 290566 hypogaea RunnerCOC249 343384 fastigiata IntermediateCOC277 259851 hypogaea VirginiaCOC294 372271 hypogaea VirginiaCOC388 162655 fastigiata SpanishCOC408 262038 fastigiata ValeniciaCOC477 268806 fastigiata SpanishCOC678 476636 hypogaea VirginiaCOC698 372305 hypogaea VirginiaCOC703 476432 fastigiata IntermediateTamrun OL02 Simpson et al. 2006 hypogaea RunnerICGS-76 Nigam et al. 1991 hypogaea VirginiaTMV-2 – fastigiata Spanish
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high-pressure sodium lamps (430 W) were used to maintaina 15/9 h light/dark photoperiod. Plants were watered welland adequately supplied with nutrients. We used a random-ized block design with three replicate blocks. During themiddle of the reproductive growth stage (67 d after plant-ing), half of the plants were subjected to water-deficit stressby withholding water for 7 d, and half of the plants con-tinued to be well watered. Prior to initiation of the waterstress, all plants were watered to saturation and pots wereweighed; the pots were covered with a gas-permeablepolyethylene sheet (ULINE, Chicago, IL, USA) to preventevaporative water loss from the soil. After 7 d, stressedplants were rewatered to saturation; on average, stressedplants used 62% of the available soil moisture. Leaves wereharvested and immediately frozen in liquid nitrogen andstored at -80 °C until further analysis.
Chlorophyll fluorescence screen forstress tolerance
A novel stress bioassay was conducted using a modifiedchlorophyll fluorescence technique described by Burke(2007). Briefly, leaf samples were collected in the glasshousebefore dawn at the end of the water stress treatment (i.e. 7 dafter water was withheld), and initial chlorophyll fluores-cence yield (Fv/Fm) measurements were conducted usingan Opti-Science OS1-FL Modulated Fluorometer (Opti-Sciences, Inc., Hudson, NH, USA). Subsequently, sampleswere maintained in a growth cabinet (40 °C) in the dark,and Fv/Fm was measured at 8, 24, 32, 48 and 72 h afterincubation. The decline in Fv/Fm over time was used as anindicator of the level of stress experienced by the plantsprior to incubation. In theory, leaves respire until theyexhaust stored carbon reserves present at the time of leafsampling. Hence, a slow decline in Fv/Fm reflected greatercarbon reserves at initial sampling, which was indicative ofhigh physiological stress and decreased sink activity. Con-versely, a rapid decline in fluorescence yield (i.e. rapid leafdeath) indicated lower physiological stress at the time ofsampling (Burke 2007).
Leaf-level photosynthesis, stomatalconductance and water-use efficiency (WUE)
At the beginning (0 d) and the end (7 d) of the water-deficitstress treatment, leaf level gas exchange was measured on arecently, fully expanded, second nodal leaf during peak pho-tosynthetic activity in midday (1000–1300 h) on peanutplants growing in the glasshouse using a portable photosyn-thesis system (Li-Cor model 6400, Lincoln, NE, USA).Leaves in the Li-Cor 6400 cuvette were maintained andmeasured under the following conditions: 38 Pa CO2,leaf temperature 27 °C, relative humidity 50–60% andsaturating photosynthetic photon flux density (PPFD)of 1900 mmol m-2 s-1 (determined by photosynthetic lightresponse curves for three plants of each genotype) providedby a blue–red LED external light source on the Li-Cor
6400 cuvette. Leaf vapour pressure deficit (DL) averaged1.86 kPa for irrigated plants and 2.34 kPa for stressedplants. Estimates of instantaneous leaf WUE were calcu-lated as the ratio of photosynthesis (A) to stomatal conduc-tance (gs).
Epicuticular wax estimation
Leaf discs (1.132 cm2) were collected from 15 well-wateredand 15 water-stressed plants at the end of the stress experi-ment. Epicuticular wax load (EWL) was estimated by bothgravimetric and colorimetric methods using the protocoldescribed by Samdur et al. (2003) and Ebercon, Blum &Jordan (1977).
Preparation of total crude protein extract andone-dimensional (1-D) gel electrophoresis(1-DGE)
Total leaf protein was extracted using the phenol extractionprotocol described by Kottapalli et al. (2008) (SupportingInformation Fig. S1). Briefly, 100 mg of lyophilized tissue,pooled from three plants, was added to an extractionmedium containing 0.9 m sucrose, 0.1 m Tris–HCl (pH 8.8),10 mm ethylenediaminetetraacetic acid (EDTA) (pH 8.0),0.4% (v/v) 2-mercaptoethanol and tris-buffered phenol (pH8.8), and gently mixed at room temperature (RT). Proteinswere precipitated by incubating the phenolic phase with0.1 m ammonium acetate–methanol at -20 °C overnight,followed by precipitation and washing of the proteins seri-ally in three organic solvents to give a highly purifiedprotein pellet. The protein content was measured by Brad-ford assay using bovine serum albumin (fraction V) as thestandard (Bradford 1976). Fifteen micrograms of proteinwas incubated for 3 min at 95 °C in sample buffer contain-ing 62 mm Tris (pH 6.8) containing 10% (v/v) glycerol,2.5% (w/v) sodium dodecyl sulphate (SDS) and 5% (v/v)2-mercaptoethanol, and a drop of bromophenol blue(BPB), then cooled to RT. After incubation on the bench(at ambient RT of 25 °C) for 10 min, the mixture wascentrifuged and the supernatant was used for SDS–polyacrylamide gel electrophoresis (SDS–PAGE, 4% T,2.6% C stacking gels, pH 6.8 and 12.5% T, 2.6% C separat-ing gels, pH 8.8). SDS–PAGE was carried out on a NihonEido (Tokyo, Japan) vertical electrophoresis unit at con-stant current of 40 mA for ca. 4 h. The running buffer wascomposed of 0.025 m Tris, 0.192 m glycine and 0.2% (w/v)SDS. Molecular mass markers (5.0 mL of the commerciallyavailable ‘ready-to-use’ Precision Plus Protein Standards,Dual Color; Bio-Rad, Hercules, CA, USA) were loaded inthe well adjacent to the samples. Gels stained with Coo-massie brilliant blue (CBB R-250) were visualized for dif-ferential banding pattern.
Immunoblotting
Electrotransfer of proteins from a gel to a polyvinyldifluo-ride (PVDF) membrane (NT-31, 0.45 mm pore size; Nihon
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Eido) was conducted at 1 mA cm-2 for 80 min at RT using asemidry blotter (Nihon Eido) as described in Rakwal et al.(2003). The ECL + plus Western Blotting Detection Systemprotocol (GE Healthcare, Little Chalfont, Buckingham-shire, UK) was used for blocking, and primary and second-ary antibody (anti-Rabbit IgG, horseradish peroxidaselinked whole antibody; from donkey) incubation. Immu-noassayed proteins were visualized on an X-ray film(X-OMAT AR, Kodak, Tokyo, Japan) using an enhancedchemiluminescence protocol (GE Healthcare).
Two-dimensional gel electrophoresis (2-DGE)
2-DGE of three selected genotypes was carried out usingIPG strip gels on an IPGphor unit followed by the seconddimension using ExcelGel XL SDS 12–14 gradient gels on aMultiphor II horizontal electrophoresis unit (GE Health-care, Piscataway, NJ, USA).The volume carrying 80 mg totalsoluble protein was mixed with LB-TT (for details, seeKottapalli et al. (2008)) containing 0.5% (v/v) pH 4.0–7.0IPG buffer (GE Healthcare) to bring to a final volume of340 mL. A trace of BPB was added and samples were cen-trifuged at 15 000 g for 15 min followed by pipetting into an18 cm strip holder tray placed into the IPGphor unit. TheIPG strips (pH 4.0–7.0; 18 cm) were placed onto the proteinsamples, avoiding air bubbles between the sample and thegel. The IPG strips were passively rehydrated with theprotein samples for 90 min, followed by overlaying the IPGstrips with cover fluid; this was directly linked to a five-stepactive rehydration and focusing protocol (18 cm strip) asdescribed previously (Hirano et al. 2007). The whole proce-dure was conducted at 20 °C, and a total of 68 902 Vh wasused for the 18 cm strip. Following IEF, the IPG strips wereimmediately used for the second dimension or stored at-20 °C.
The strip gels were incubated twice in equilibrationbuffer containing 50 mm Tris–HCl (pH 8.8), 6 m urea, 30%(v/v) glycerol, 2% (w/v) SDS and 2% (w/v) dithiothreitol(DTT) for 10 min with gentle agitation, followed by incu-bation in the same equilibration buffer supplemented with2.5% (w/v) iodoacetamide for 10 min at RT. For horizontalelectrophoresis, 18 cm IPG strips were placed onto theSDS 12–14% gradient gels after equilibration, followed byplacement of the cathode and anode buffer strips andelectrodes, respectively. SDS–PAGE (20 and 40 mA/gel)was performed as per manufacturer recommendations(GE Healthcare). Molecular masses were determined byrunning Dual Color Precision plus Protein Standard proteinmarkers (Bio-Rad); for each sample, a minimum of fourIPG strips and corresponding SDS–PAGE was used underthe same conditions.
Protein visualization, image analysis andspot quantification
To visualize the protein spots, the polyacrylamide gels werestained with CBB. Protein patterns in the gels were
recorded as digitized images using a digital scanner (CanonCanoScan 8000F, resolution 300 dpi, 16-bit grayscale pixeldepth) and saved in tagged image file formats.The gels werequantified in profile mode using ImageMaster 2D Platinumsoftware version 5.0 (GE Healthcare, Little Chalfont,Buckinghamshire, UK). Protein abundance was expressedas relative volume according to the normalization methodprovided by ImageMaster software that compensates forgel-to-gel variation in sample loading, gel staining anddestaining (Agrawal & Thelen 2005; Hajduch et al. 2005). Inorder to analyse differences in relative protein abundance,spot volumes were compared with those of correspondingspots in fully irrigated control samples; spot differenceswere also manually confirmed. Moreover, the CBB-stainedspots were selected for comparative profiling only if theywere confirmed in three independent gel replications.
Spots that exhibited � 1.5-fold difference (in all three gelreplications) in relative abundance in water-stressed plantscompared to well-watered plants were selected for massspectrometry analysis. Additionally, the protein bandsfrom 1-D gels showing differential accumulation betweensamples were excised along with the corresponding bandsfrom control sample lanes and transferred to sterile 1.5 mLtubes. Distinct differentially expressed protein spots fromtwo-dimensional (2-D) gels were picked using a gel picker(One Touch Spot Picker, P2D1.5 and 3.0;The Gel Company,San Francisco, CA, USA); excised bands/spots were storedat -30 °C.
Protein identification using mass spectrometry
Proteins were identified using peptide mass fingerprinting(PMF) methods (Jensen et al. 1997) utilizing mass spec-trometry. In the PMF method, excised gel spots weredestained with 100 mL of destain solution (30 mm potassiumferricyanide in 100 mm sodium thiosulphate), with shakingfor 5 min. After the solution was removed, gel spots wereincubated with 200 mm ammonium bicarbonate (hereafterrefered to as AMBIC) for 20 min. Gel pieces were dried ina speed vacuum concentrator for 5 min and then rehy-drated with 20 mL of 50 mm AMBIC containing 0.2 mgmodified trypsin (Promega, Madison, WI, USA) for 45 minon ice. After removal of solution, 30 mL of 50 mm AMBICwas added, and the digestion was performed overnight at37 °C. The peptides were desalted and concentrated usingC18 nanoscale (porous C18) columns (IN2GEN, Seoul,Korea). In preparation for use in the matrix-assisted laserdesorption/ionization–time-of-flight mass spectrometer(MALDI–TOF MS), peptides were eluted by 0.8 mL ofmatrix solution (70% acetonitrile, 0.1% TFA, 10 mg mL-1
alpha-cyano-4-hydroxycinnamic acid) and then spottedonto a stainless steel target plate. Masses of peptides weredetermined using MALDI–TOF MS (model MALDI-R;Micromass, Manchester, UK); calibration was performedusing internal mass of trypsin auto digestion product(m/z 2211.105).
In preparation for analysis by quadrupole time-of-flighttandem mass spectrometry (Q-TOF MS/MS), 15 mL of the
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peptide solution from the digestion supernatant was dilutedwith 30 mL in 5% formic acid, loaded onto the column andwashed with 30 mL of 5% formic acid. Peptides were elutedwith 2.0 mL methanol/H2O/formic acid (50/49/1, v/v/v)directly into a precoated borosilicate nanoelectrosprayneedle (EconoTip; New Objective, Inc., Woburn, MA,USA). MS/MS of peptides generated by in-gel digestionwas performed by nano-ESI on a Q-TOF2 MS using asource temperature of 80 °C. A potential of 1 kV wasapplied to the precoated borosilicate nanoelectrosprayneedles in the ion source combined with a nitrogenback-pressure of 0–5 psi to produce a stable flow rate(10–30 nL min-1). The Q-TOF2 MS was operated in anautomatic data-dependent mode to collect ion signals fromthe eluted peptides. In this mode, the most abundantpeptide ion peak with doubly or triply charged ion in afull-scan mass spectrum (m/z 400–1500) was selected as theprecursor ion. Finally, an MS/MS spectrum was recorded toconfirm the sequence of the precursor ion using collision-induced dissociation (CID) with a relative collision energydependant on molecular weight; cone voltage was 40 V.Thequadrupole analyser was used to select precursor ions forfragmentation in the hexapole collision cell. The collisiongas was Ar at a pressure of 6–7 ¥ 10-5 mbar, and the collisionenergy was 20–30 V. Product ions were analysed using anorthogonal TOF analyser, fitted with a reflector, a micro-channel plate detector and a time-to-digital converter; datawere processed using a MassLynx (ver. 3.5) Windows NTPC system.
Protein identification was performed by searchingthe National Center for Biotechnology Information(NCBI) non-redundant database using the MASCOTsearch engine (Matrix Science, London, UK; http://www.matrixscience.com), which uses a probability-basedscoring system. The following parameters were used fordatabase searches (NCBInr 20070120, 4462937 sequences;1534242322 residues) with MALDI–TOF PMF data:trypsin as digesting enzyme, carbamidomethylation ofcysteine as a fixed modification, oxidation of methionineas variable modification, monoisotopic mass, unrestrictedprotein mass, � 100 ppm peptide mass tolerance, 1+peptide charge state, with one missed cleavage allowed.For MALDI–TOF MS data to qualify as a positive iden-tification, a peptide score had to equal or exceed theminimum significant score. For database searches(NCBInr 20070127, 4496228 sequences; 1544738466 resi-dues; Taxonomy Viridiplantae, 283484 sequences) withMS/MS spectra, the following parameters were used:trypsin as digesting enzyme, carbamidomethylationof cysteine as a fixed modification; oxidation of methion-ine as allowable variable modifications, monoisotopicmass value and unrestricted protein mass; � 1.0 Dapeptide mass tolerance and � 0.8 Da fragment mass tol-erance; peptide charge of +1, +2 or +3; with one missedcleavage allowed. Positive identification of proteins byMS/MS analysis required a minimum of two unique pep-tides, with at least one peptide having a significant ionscore.
Gene expression analysis usingreal-time qRT-PCR
Total RNA from leaf tissue was isolated using the RNeasyPlant Mini-kit (Qiagen, Valencia, CA, USA). Leaves wereground to a fine powder in liquid nitrogen, and approxi-mately 100 mg of homogenized tissue was used for totalRNA isolation. RNA samples were treated with TurboDNAfree (Ambion, Austin, TX, USA) prior to cDNA syn-thesis. One microgram of total RNA was used to synthesizefirst-strand cDNA using the SuperScript First StrandSynthesis system for RT-PCR (Invitrogen, Carlsbad, CA,USA). The primers for eight candidate proteins identifiedfrom this study were designed using Integrated DNA Tech-nologies primer designing tools (see Supporting Informa-tion Table S1). The efficiency of the primer pairs wasdetermined using cDNA derived from the irrigated samplesusing a 1:2 serial dilution series. Primer efficiency reactionswere performed in triplicate in a volume of 25 mL usingSuperArray SYBRGreen reaction mix (SuperArray Bio-science Corp., Frederick, MD, USA).
Reactions were subjected to real-time qRT-PCR usingthe Roche LightCycler 480 Real-Time PCR System andanalysed using the LightCycler 480 quantification software(Roche Biochemicals, Indianapolis, IN, USA). Sampleswere analysed in a 25 mL reaction volume using the RocheLightCycler. Reactions were performed in triplicate usingcDNA templates from treated and control samples for eachgene (candidate genes and actin-DF gene). A master mix ofSYBRGreen and primers was prepared for each primerpair. RT-PCR reactions were performed on 40 ng totalRNA with 400 nm specific primers under the followingconditions: one cycle of denaturation at 95 °C for 10 minfollowed by 40 cycles each consisting of 95 °C for 15 s(denaturation) and 60 °C for 15 s (annealing and elonga-tion). The PCR reaction was followed by a melting curveprogramme (60–95 °C with a heating rate of 0.1 °C s-1 and acontinuous fluorescence measurement) and then a coolingprogramme at 40 °C. Negative controls lacking reversetranscriptase were run with all reactions. PCR productswere also run on agarose gels to confirm the formation of asingle product at the desired size. Crossing points for eachtranscript were determined using the second-derivativemaximum analysis with the arithmetic baseline adjustment.Crossing point values for each gene were normalized to therespective crossing point values for the reference geneactin-DF. Data were presented as normalized ratios ofgenes along with error standard deviations estimated usingthe Roche Applied Science E-method (Tellmann & Geulen2006).
Statistical analyses
Each experiment was replicated at least three times. Valuesare expressed as means � SE. Data were analysed usingKaleidaGraph (Synergy Software, Reading, PA, USA) soft-ware. All mean comparisons were done using t-test forindependent samples. For photosynthetic rate and stomatal
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conductance, the different measurements were subjected toa one-way analysis of variance (anova). Confidence coeffi-cient a in all cases was set at 0.05.
RESULTS AND DISCUSSION
Screening of US peanut mini-core genotypesfor water-deficit stress tolerance
We evaluated 17 genotypes from the US peanut mini-corecollection and three check cultivars using the chlorophyllfluorescence screening technique following imposition ofwater-deficit stress. Of these 20 genotypes, we identifiedfive stress-tolerant (COC041, COC384, COC249, COC149,TMV-2) and five stress-susceptible (COC166, COC227,COC068, Tamrun OL02, ICGS 76) genotypes based onobservations of chlorophyll fluorescence yield (Fig. 1a),whole-plant WUE (mg mass produced per g of water used;Fig. 1b), and specific leaf area (SLA; cm2 leaf area per g leafmass; Fig. 1c). Tolerant genotypes were characterized bysmaller percentage changes in chlorophyll fluorescenceyield during water-deficit stress, higher WUE during well-watered and deficit stress conditions and slightly higherSLA, compared with susceptible genotypes. The most toler-ant genotype (COC041) exhibited a similar decline in fluo-rescence yield over time in both water-stressed and well-watered plants (Fig. 1d). In contrast, the most susceptiblegenotype (COC166) exhibited a marginal decline in fluo-rescence yield in the water-stressed plants after 72 h ofincubation.The tolerant genotype (COC041) also exhibitedhigher whole plant WUE than the susceptible genotype(COC166).
Our results indicate that the elevated respiratory demandbioassay, designed to measure source leaf responses toabiotic stresses in cotton (Burke 2007), can be employed toscreen peanut genotypes for divergence in response towater-deficit stress. Here, we have designated COC041 as astress-tolerant genotype and COC166 as stress susceptiblebased on higher relative whole-plant WUE and normalchlorophyll fluorescence under stress conditions comparedto other selected US mini-core accessions and check culti-vars during water-deficit stress. As further confirmation ofour designation of COC041 as a tolerant genotype andCOC166 as susceptible, we compared the yield of thesegenotypes under field conditions of full and moderatedeficit irrigation of approximately 100 and 70% potentialevapotranspiration (PET) replacement, respectively. Whengrown in deficit irrigation conditions of 70% PET, the sus-ceptible genotype exhibited approximately 90% decline inyield, while the tolerant genotype exhibited a 15–20%decline in yield compared to the 100% PET treatment(Fig. 2a,b).
Leaf physiological responses to water stress
Figure 3 shows that light-saturated photosynthesis (A)was similar in the tolerant (COC041) and susceptible(COC166) genotypes before water stress was applied (0 d)
and at the end of the stress period (7 d), but A was higherin the susceptible genotype during stress exposure (3 d)because of higher stomatal conductance (gs; Table 2). Onthe second day after rewatering, A and gs were higher inthe tolerant genotype reflecting faster recovery fromstress, but 7 d after rewatering both genotypes had fullyrecovered (Table 2). Instantaneous leaf-level WUE (A/gs;WUE) was higher in the tolerant genotype prior to andduring the onset of water deficit because of lower gs.However, upon return to saturated soil moisture condi-tions, assimilation rates and stomatal conductanceincreased rapidly (within 48 h), and WUE was lower in thetolerant genotype compared to the susceptible genotype.Although the susceptible genotype showed a slowerrecovery following the stress treatment, both genotypesrecovered to pre-stress levels of photosynthesis 7 d afterrewatering (Table 2). In general, the response to soil mois-ture availability is significantly faster in the tolerant geno-type compared to susceptible plants, and this appears tobe, in part, caused by better stomatal control.
Differences in protein profiles between tolerantand susceptible genotypes
1-DGE was used to identify broad protein-level differencesbetween the tolerant and susceptible genotypes and thecheck cultivar. On 12.5% SDS–PAGE gels, 43 differentialbands were observed in the tolerant genotype (COC041),susceptible genotype (COC166) and check cultivar(TMV2) under well-watered and water-deficit conditions(Fig. 4). Only those bands showing distinct differencesbetween stressed and well-watered samples (23 in total)were selected for LC-MS/MS analysis, generating the iden-tification of 17 non-redundant proteins (Table 3).
Changes in protein profiles in the susceptible, tolerantand check cultivar peanut plants during water stress wereobserved in 2-DGE analysis of total proteins (Fig. 5). Quan-titative image analysis indicated 79 differential proteinspots exhibited significantly altered intensities (� 1.5-foldover well-watered control) in water-stressed plants. These79 differential proteins were then analysed by MALDI–TOF MS and Q-TOF MS/MS, and 48 non-redundant pro-teins with altered intensities were observed (� 1.5-fold overwell-watered control) in water-stressed plants (Table 4).Spectra of all proteins identified by MALDI and Q-TOFare provided in our peanut protein database (http://www.lbk.ars.usda.gov/psgd/index-peanut.aspx).
We categorized these proteins into 10 different knownfunctional groups (representing 83% of proteins) and one,relatively small unknown group (13% of proteins; Fig. 6).Surprisingly, the identities of very few differentiallyexpressed proteins were unknown. This may be because ofthe fact that majority of abundant leaf proteins have beenwell characterized (Larrainzar et al. 2007).The largest func-tional groups were proteins associated with photosynthesis(25%), lectins (15%), signal transduction (13%) and waterstress (10%). Apart from the known enzymes involvedin photosynthesis, five proteins implicated in signal
Physiology and proteomics of the water-deficit stress response 385
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
0
10
20
30
40
50
60
70
80
90
100 Water-deficit stressWell watered
Flu
ores
cenc
e yi
eld
(% c
hang
e)
COC166 COC227 COC149 COC249 COC384 COC041COC068 TMV-2TamrunOL02
ICGS 76
0.0
1.0
2.0
3.0
4.0
5.0
6.0
7.0
8.0
COC166 COC227 COC068 ICGS 76 TamrunOL02
COC149 COC249 COC384 COC041 TMV-2
Water-deficit stressWell watered
WU
E(m
g bi
omas
s g–
1 H
2O)
SLA
(cm
2 /10
0mg)
Water-deficit stressWell watered
0.0
0.5
1.0
1.5
2.0
2.5
3.0
3.5
4.0
4.5
COC166 COC227 COC068 ICGS 76 TamrunOL02
COC149 COC249 COC384 COC041 TMV-2
(a)
(b)
(c)
Figure 1. (a) Percent change in chlorophyll fluorescence yield for 10 selected peanut genotypes exposed to slow-onset water-deficitstress for 7 d. The chlorophyll fluorescence values indicate the percent change in yield at 72 h compared to 0 h. (b) Water-use efficiency(WUE) calculated as the ratio of biomass produced per given amount of water (mg g-1). (c) Specific leaf area (SLA) given as ratio of leafarea and leaf dry mass (cm2 100 mg). (d) Graphs showing time-course chlorophyll fluorescence yield decline of control (white squares)and water-stressed (black squares) source leaves of peanut genotypes COC041 and COC166, and cultivar TMV2.
386 K. R. Kottapalli et al.
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
transduction were detected during water stress (Tables 3and 4). These included lipoxygenase (LOX) (Table 3, band5), cyclophilin (Table 3, band 14), calmodulin-bindingprotein (CBP) (Table 3, band 15), nucleoside diphosphatekinase 1 (NDK1) (Table 3, band 16) and 1l-myo-inositol-1-phosphate synthase (Table 4, spot 30). Levels of LOXprotein increased during water stress in tolerant genotypes.Fatty acid hydroperoxide-like linolenic acid produced byLOX is a precursor for biosynthesis of jasmonic acid, asignalling molecule that activates plant defence mecha-nisms (Lee et al. 2005). It is possible that jasmonic acid,produced by lipoxygenase, may be involved in perceptionand transduction of extracellular signals during water stress.However, it should be noted that the role of LOX in thestress response is complex (Fauconnier et al. 2002), and thepossible involvement of jasmonic acid, here, requiresfurther investigation. On the other hand, the increase in1l-myo-inositol-1-phosphate synthase during stress sug-gests its indirect involvement in water stress signallingthrough phosphoinositoids. 1l-Myo-inositol-1-phosphate
synthase catalyses the reaction from glucose-6-phosphateto inositol-1-phosphate [I(1)P], the first step of myo-inositolbiosynthesis. Phosphoinositides synthesized from I(1)P areplasma membrane-bound proteins and involved in signaltransduction (Yoshida et al. 1999).
Previous studies showed that nucleoside diphosphatekinases (NDKs) play a role in GTP-mediated signal trans-duction pathways, light response and reactive oxygen scav-enging, and are involved in plant response to heat andwater deficit (Pan et al. 2000; Galvis et al. 2001; Fuka-matsu, Yabe & Hasunuma 2003; reviewed by Hasunumaet al. 2003; Hajheidari et al. 2005; Bhushan et al. 2007).NDK1 protein was highly induced under water-deficitstress in sweet potato (Hajheidari et al. 2005), but itsexpression was reduced in a stress-tolerant chickpea cul-tivar grown under water-deficit stress (Bhushan et al.2007). Interestingly, in our study, levels of NDK1 proteinincreased only in the susceptible genotype in response towater-deficit stress (Table 3, band 16). Contrastingly,NDK1 levels decreased in response to water deficit in the
0.1
0.2
0.3
0.4
0.5
0.6
0.7
0.8
0.9
0 10 20 30 40 50 60 70 80
COC041(tolerant)
Water-deficit stressWell watered
Fv/
Fm
Fv/
Fm
Time at 40 °C
TMV-2(tolerant)
Time at 40 °C
0.1
0.2
0.3
0.4
0.5
0.6
0.7
0.8
0.9
0 10 20 30 40 50 60 70 80
0.1
0.2
0.3
0.4
0.5
0.6
0.7
0.8
0.9
0 10 20 30 40 50 60 70 80
COC166(susceptible)
Time at 40 °C
(d)
Water-deficit stressWell watered
Water-deficit stressWell watered
Fv/
Fm
Figure 1. Continued.
Physiology and proteomics of the water-deficit stress response 387
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
tolerant cultivar TMV2 and could not be detected in thetolerant COC041 genotype plants. Whether this indicatesthat COC041 leaves were not under the same level ofwater-deficit stress experienced by TMV2 and COC166 oran alternative mechnism or absence of this protein in
COC041 is unknown. However, transcript for this genewas induced in all three genotypes in response to water-deficit stress.
The cyclophilin protein was induced both in the suscep-tible genotype and the TMV2 cultivar, and remained
(a)
(b)
0
4
8
12
16
20
24
28
32
36
40
COC166
COC041
Control 50% Irrigation
seed
yie
ld(g
pla
nt–1
)
*
*
COC041COC166
70% PET replacement 100% PET replacement
70% PET replacement 100% PET replacement
Figure 2. (a) Comparison of pod yield for COC166 (top panel) and COC041 (bottom panel) grown under deficit irrigation [70%potential evapotranspiration (PET) replacement] in 2008 field trials conducted at the ARS Cropping Systems Laboratory in Lubbock, TX,USA. (b) Under moderate water-deficit conditions, COC166 shows approximately 90% decrease in pod yield, while COC041 showsroughly a 22% decrease in yield compared to fully irrigated plants. Statistically significant differences were measured for all comparisons,and those were P < 0.001 are indicated as *.
388 K. R. Kottapalli et al.
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
unchanged in the tolerant COC041. Cyclophilins differen-tially expressed during water stress are involved in a varietyof cellular processes. Besides protein folding function, theyalso play a role in signal transduction and thus may becrucial for stress responsiveness (Romano, Horton & Gray2004). In sugarbeet and sorghum, cyclophilins wereaccumulated in the tolerant cultivars during water-deficitstress (Hajheidari et al. 2005). However, in chickpea, thecyclophilin-like peptidyl-prolyl cis-trans isomerase wasreduced during dehydration in the tolerant cultivar
(Bhushan et al. 2007). Our work with peanuts and that ofBhushan et al. (2007) with chickpeas suggest negative sig-nalling of cyclophilins in these two legume species. Anothersignalling protein, calmodulin, is a ubiquitous calciumreceptor that regulates the activities and functions of a widerange of CBPs. A significant increase in the protein wasseen in the susceptible genotype and may be involved informing complexes with CBP like GAD or protein kinases(Fromm & Snedden 1997) required for calcium signalling inresponse to water-deficit stress. Absence of induction of the
0.0
5.0
10.0
15.0
20.0
25.0
30.0
Beg
inir
riga
tion
(rec
over
y)
Stop
irri
gati
on
Day 0(100%)
Day 3 Day 7(40%)
Day 2(100%)
Day 7(100%)
A (mm
ol C
O2
m–2
s–1
)
Irrigation treatment
**
*
**
Figure 3. Photosynthetic response to water-deficit stress in COC041 (black bars) and COC166 (white bars). Data are mean values of netphotosynthesis � SEs (n � 6 for each measurement). Statistically significant differences are indicated as **P � 0.01 and *P � 0.05.
Table 2. Stomatal conductance (gs; mol H2O m-2 s-1), transpiration (E; mmol H2O m-2 s-1) and estimates of water-use efficiency (WUE)(A/gs and A/E) for COC041 and COC166 plants exposed to slow-onset water-deficit stress for 7 d followed by rewatering to soilsaturation daily for 7 d
gs E A/gs A/E
COC041 COC166 COC041 COC166 COC041 COC166 COC041 COC166
Water deficitDay 0 0.412 0.478 6.28 9.58 52.9 40.8** 4.4 2.1*
(0.026) (0.08) (1.02) (1.29) (9) (1.8) (1) (0.1)Day 3 0.102 0.142 3.39 4.69* 115.4 112.9* 3.4 3.4
(0.007) (0.018) (0.2) (0.53) (5.3) (5.3) (0.2) (0.2)Day 7 0.063 0.069 1.78 2.04 152.8 139.8** 5.7 5.1
(0.007) (0.009) (0.17) (0.25) (4.7) (4.9) (0.5) (0.8)RewaterDay 2 0.316 0.188** 7.78 4.61** 52.1 88.2** 2 2.9*
(0.06) (0.101) (0.62) (0.15) (4.4) (5) (0.2) (0.2)Day 7 0.458 0.655*** 9.4 11.72*** 54.2 42.8* 2.6 2.3
(0.046) (0.04) (0.59) (0.41) (4.2) (2.1) (0.1) (0.1)
Data are mean values with SEs in parentheses (n � 6).Statistically significant differences are indicated at ***P � 0.001, **P � 0.01 and *P � 0.05.
Physiology and proteomics of the water-deficit stress response 389
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
protein in tolerant genotype COC041 suggests that eitherthe plants are not experiencing the same level of stress or apossible mechanism to avoid stress by blocking the trans-mission of signals to CBP.
Interestingly, a tetratricopeptide repeat containingprotein (TPR) (Table 4, spot 78), a positive regulator ofABA signalling during plant development under stress was
induced in the tolerant line and check cultivar with thelatter showing more specific induction of the protein(Fig. 5). The TPR-containing proteins were shown to bestress responsive in soybean under heat stress (Torres, Cha-tellard & Stutz 1995) and Arabidopsis in response to saltand osmotic stress (Rosado et al. 2006). The ArabidopsisTPR-containing TTL1 mutants have reduced tolerance tosalt and osmotic stress, characterized by reduced root elon-gation and disorganization of the root meristem. It was alsoshown that TTL1 regulates the transcript levels of severaldehydration-responsive genes including the transcriptionfactor DREB2A (Rosado et al. 2006). Further, it was dem-onstrated that TTL1 acts as a positive regulator of ABAsignalling during plant development under stress. Thus,TPR-containing proteins may function as members of mul-tiprotein complexes implicated in the regulation of ABAsignalling and abiotic stress responses in the tolerant peanutgenotype.
Our proteomics analysis also identified proteins involvedin ameliorating water stress. Methionine synthase (Table 4,spot 1), the enzyme responsible for synthesis of S-adenosylmethionine (SAM), was reduced in all three genotypesduring water deficit. Lignification of the cell wall by methy-lation of lignin monomers may be one mechanism to avoidwater loss under dehydration (Bhushan et al. 2007). Addi-tionally, changes in phenylpropanoid biosynthesis, namelymethylation of lignin precursors by S-adenosyl methioninesynthetase and the production of ferulic acid represent keysteps in cell wall lignification and cell expansion (Chazenand Neumann 1994; Neuman 1995; Riccardi et al. 1998). Inthis reaction, SAM serves as the primary methyl groupdonor. Cellular levels of SAM are regulated by the activityof methionine synthase which generates methionine, aprecursor of SAM (Ravanel et al. 1998, 2004). Induction ofmethionine synthase transcript suggests an increased pro-duction of methionine and lignin methylation by SAM. Onthe other hand, reduction of the protein under water stressin all accessions may be caused by a demand for moremethyl groups for lignin methylation.
For proteins involved in photorespiration, we detectedglycine dehydrogenase (decarboxylating) (Table 3, band17), which was induced in the susceptible genotype duringwater stress.The glycine dehydrogenase enzyme family con-sists of glycine cleavage system P-proteins EC 1.4.4.2 frombacterial, mammalian and plant sources. The P protein ispart of the glycine decarboxylase (GDC; EC 2.1.2.10) multi-enzyme complex, and catalyses the interconversion ofglycine to serine, an integral part of the photorespiratorypathway (Bauwe & Kolukisaoglu 2003). It has been sug-gested that decreased GDC in pea mitochondria followingexposure to water-deficit stress is a result of oxidativedamage and that GDC inhibition may serve as an initialmarker of oxidative stress in plant cells (Taylor, Day &Millar 2002). Reduction of this protein in TMV2 mayindicate damage to the photorespiratory pathway duringwater-deficit stress, while increased expression of GDC insusceptible plants suggests the possible involvement ofphotorespiration as an electron sink in minimizing reactive
1-DGE
1
15 mg
M
12.5
% S
DS
–PA
GE
250
150
100
75
50
37
25
20
15
2 3 4 5 6
LSU
SSU
1
345
7
68
9
10
111213
1516
1718
19
2021
222324
252627
282930
14 31
32
3334
3536
3738
394041
42
43
(kDa)
2A 2B 2C
Figure 4. Coomassie brilliant blue (CBB)-stainedone-dimensional (1-D) gel protein profiles of leaves from controland water-stressed plants (equal protein amounts ca. 15 mg wereapplied) was carried out as described in Materials and methods.Leaf proteins from COC041 control (1), COC041 water stresstreated (2), COC166 control (3), COC166 water stress treated(4), TMV2 control (5), TMV2 water stress treated (6) werementioned above each lane. Molecular weights (kDa) of proteinmarkers (Precision Plus Protein Standards) are indicated at theleft. Sodium dodecyl sulphate–polyacrylamide gel electrophoresis(SDS–PAGE) (4% T, 2.6% C stacking gels, pH 6.8 and 12.5% T,2.6% C separating gels, pH 8.8) was carried out using 12.5%polyacrylamide gels on a Nihon Eido (Tokyo, Japan) verticalelectrophoresis unit at constant current of 40 mA for ca. 4.5 h.The running buffer was composed of 0.025 m Tris, 0.192 m glycineand 0.2% (w/v) SDS. Five microlitres of the commerciallyavailable ‘ready-to-use’ molecular mass standards (Precision PlusProtein Standards, Dual Color) was loaded in the well adjacentto the samples.
390 K. R. Kottapalli et al.
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
Tab
le3.
Pea
nut
leaf
prot
ein
iden
tific
atio
nby
tand
emm
ass
spec
trom
etry
(MS)
from
silv
erni
trat
e-st
aine
dpr
otei
nba
nds
visu
liaze
don
one-
dim
ensi
onal
gele
lect
roph
ores
is(1
-DG
E)
Ban
dN
o.Tr
eatm
ent
Pro
tein
iden
tifie
dR
elat
ive
abun
danc
e1
23
45
6Sc
ore
Sequ
ence
cove
rage
Acc
essi
onP
epti
de
1C
ontr
olTy
peII
Ich
loro
phyl
la/b
-bin
ding
prot
ein
12
34
56
485
gi|2
0794
YA
ML
GA
VG
AIA
PE
ILG
K
Con
trol
Car
boni
can
hydr
ase,
chlo
ropl
ast
prec
urso
r(C
arbo
nate
dehy
drat
ase)
EC
4.2.
1.1
475
gi|1
1547
2E
AV
NV
SLG
NL
LTY
PF
VR
WS
Oxy
gen-
evol
ving
enha
ncer
prot
ein
2,ch
loro
plas
tpr
ecur
sor
(OE
E2)
768
gi|1
3139
0SI
TD
YG
SPE
EF
LSK
VD
YL
LG
K
WS
Car
boni
can
hydr
ase,
chlo
ropl
ast
prec
urso
r(C
arbo
nate
dehy
drat
ase)
EC
4.2.
1.1
605
gi|1
1547
2E
AV
NV
SLG
NL
LTY
PF
VR
2AC
ontr
olR
ibul
ose-
1·5-
biph
osph
ate
carb
oxyl
ase-
oxyg
enas
elar
gesu
buni
t
12
34
56
309
–gi
|234
2884
@
WS
AT
Psy
ntha
sebe
tasu
buni
tE
C3.
6.3.
1439
1–
gi|1
6943
747
@
2BC
ontr
olA
TP
synt
hase
beta
subu
nit
219
–gi
|147
1796
2
WS
AT
Psy
ntha
sebe
tasu
buni
tE
C3.
6.3.
1417
2–
gi|7
7082
86@
WS
Rib
ulos
e-1·
5-bi
phos
phat
eca
rbox
ylas
e-ox
ygen
asel
arge
subu
nit
188
–gi
|170
6618
3@
2CC
ontr
olA
TP
synt
hase
beta
subu
nit
179
–gi
|500
1575
@
Con
trol
Rib
ulos
e-1·
5-bi
phos
phat
eca
rbox
ylas
e-ox
ygen
asel
arge
subu
nit
172
–gi
|234
2884
@
WS
AT
Psy
ntha
sebe
tasu
buni
tE
C3.
6.3.
1428
5–
gi|6
6276
267
@
WS
Rib
ulos
e-1·
5-bi
phos
phat
eca
rbox
ylas
e-ox
ygen
asel
arge
subu
nit
268
–gi
|177
0291
@
3C
ontr
olC
arbo
nic
anhy
dras
e,ch
loro
plas
tpr
ecur
sor
(Car
bona
tede
hydr
atas
e)
12
34
56
315
gi|1
1547
2E
AV
NV
SLG
NL
LTY
PF
VR
Con
trol
751(
+2)
–M
S/M
S,pe
rmea
sepr
otei
nof
suga
rA
BC
tran
spor
ter
6690
**Q
98JY
6E
YN
LL
PD
HLV
G**
*
WS
Car
boni
can
hydr
ase,
chlo
ropl
ast
prec
urso
r(C
arbo
nate
dehy
drat
ase)
EC
4.2.
1.1
535
gi|1
1547
2E
AV
NV
SLG
NL
LTY
PF
VR
WS
Unk
now
nN
DN
DN
DA
LSP
HV
LD
WR
ALV
MA
MR
*
4C
ontr
olH
eat
shoc
kpr
otei
n81
-1(H
SP81
-1)
(Hea
tsh
ock
prot
ein
82)
12
34
56
422
gi|4
1715
4G
IVD
SED
LP
LN
ISR
WS
Unk
now
nN
DN
DN
DLT
TSL
DG
VT
AY
NA
L
5C
ontr
olP
hosp
holip
ase
D
12
34
56
221
gi|1
6988
44L
EG
PIA
WD
VL
FN
FE
QR
WS
Lip
oxyg
enas
eE
C1.
13.1
2.11
302
gi|4
3985
7Y
GPA
KM
PY
TL
LYP
SSE
EG
LTF
R
WS
1125
(+2)
–M
S/M
S,Se
edlip
oxyg
enas
e-1
(EC
1.13
.11.
12)
(L-1
)88
91**
P08
170
KP
NE
DY
PY
AA
DG
LE
LA
DG
AL
K**
*
Physiology and proteomics of the water-deficit stress response 391
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
Tab
le3.
Con
tinue
d
Ban
dN
o.Tr
eatm
ent
Pro
tein
iden
tifie
dR
elat
ive
abun
danc
e1
23
45
6Sc
ore
Sequ
ence
cove
rage
Acc
essi
onP
epti
de
6C
ontr
olG
lyce
rald
ehyd
e-3-
phos
phat
ede
hydr
ogen
ase,
cyto
solic
12
34
56
848
gi|1
2066
6A
ASF
NII
PSS
TG
AA
K,
LVSW
YD
NE
WG
YST
R
Con
trol
Ald
olas
e70
12gi
|169
039
TV
VSI
PN
GP
SAL
AV
K,
YA
AIS
QD
NG
LVP
IVE
PE
ILL
DG
EH
GID
R
WS
Gly
cera
ldeh
yde-
3-ph
opha
tede
hydr
ogen
ase,
cyto
solic
EC
1.2.
1.12
135
10gi
|120
666
GIL
GY
TE
DD
VV
STD
FV
GD
SR,
LVSW
YD
NE
WG
YST
R
7C
ontr
ol91
8(+2
)–
MS/
MS,
Ant
i-H
(O)
lect
inI
(CSA
-I)
12
34
56
2591
**P
2297
0E
LQ
DG
LTF
FL
APA
LSS
K**
*
WS
918(
+2)
–M
S/M
S,A
nti-
H(O
)le
ctin
I(C
SA-I
)57
76**
P22
970
QN
AG
DG
LTF
ML
APA
S***
8C
ontr
olO
xyge
n-ev
olvi
ngen
hanc
erpr
otei
n1,
chlo
ropl
ast
prec
urso
r(O
EE
1)
12
34
56
699
gi|1
1134
054
ITL
SVT
QSK
PE
TG
EV
IGV
FE
SIQ
PSD
TD
LG
AK
Con
trol
810(
+3)
–M
S/M
S,36
kDa
oute
rm
itoc
hond
rial
mem
bran
epr
otei
n(p
orin
)66
90**
P42
056
SSN
EN
TLT
LG
YA
N**
*
WS
1132
(+2)
–M
S/M
S,sa
me
asco
ntro
l,U
nkno
wn
10C
ontr
olC
hlor
ophy
lla/
b-bi
ndin
gpr
otei
nof
LH
CII
type
I,ch
loro
plas
tpr
ecur
sor
(CA
B)
(LH
CP
)
12
34
56
4413
gi|1
1576
8IA
GG
PL
GE
VT
DP
IYP
GG
SF
DP
LG
LA
DD
PE
AFA
EL
K
Con
trol
870(
+2)
–M
S/M
S,C
hlor
ophy
lla/
b-bi
ndin
gpr
otei
n63
80**
AB
E80
774
AT
PF
QP
YSE
VF
VA
QR
***
WS
870(
+2)
–M
S/M
S,C
hlor
ophy
lla/
b-bi
ndin
gpr
otei
n**
WS
729(
+2)
–M
S/M
S,L
ecti
npr
ecur
sor
6080
**Q
5ZE
W9
VL
AV
EM
DT
FF
DR
***
WS
897(
+2)
–M
S/M
S,M
anno
se/
gluc
ose-
bind
ing
lect
inpr
ecur
sor
(Fra
gmen
t)62
69**
Q43
376
SCH
SLN
VLV
TY
DG
SSR
***
392 K. R. Kottapalli et al.
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
11C
ontr
olM
ajor
Cab
prot
ein
12
34
56
8027
gi|1
6919
3P
GG
SFD
PL
GL
AD
DP
EA
FAE
LK
Con
trol
Chl
orop
hyll
a/b-
bind
ing
prot
ein
ofL
HC
IIty
peI,
chlo
ropl
ast
prec
urso
r(C
AB
)(L
HC
P)
6813
gi|1
1576
8IA
GG
PL
GE
VT
DP
IYP
GG
SF
DP
LG
LA
DD
PE
AFA
EL
K
WS
LH
CII
type
Ich
loro
phyl
la/b
-bin
ding
prot
ein
9719
gi|9
5872
07W
AM
LG
AL
GSV
FP
EL
LA
R,
IAG
GP
LG
EV
TD
PIY
PG
GSF
DP
LG
LA
DD
PE
AFA
EL
K
12C
ontr
olFa
iled
12
34
56
WS
Cyt
opla
smic
ribo
som
alpr
otei
nL
1868
5gi
|606
970
AP
LG
QN
TV
LL
R
WS
Pep
tide
751
m/z
–P
erm
ease
prot
ein
ofsu
gar
AB
CQ
98JY
6W
TA
AA
SYA
LA
LA
TSP
K**
WS
811(
+2)
–M
S/M
S,U
nkno
wn
LTP
DY
DA
LD
VA
NK
LG
LL
**
13C
ontr
ol91
6(+2
)–
MS/
MS,
60S
ribo
som
alpr
otei
nL
23a
(L25
)
12
34
56
WS
60S
ribo
som
alpr
otei
nL
23a
(L25
)39
11gi
|585
876
LTP
DY
DA
LD
VA
NK
IGII
WS
698(
+2)
–M
S/M
SN
GG
LYM
LL
GT
LG
**
14C
ontr
olC
yclo
phili
n
12
34
56
596
gi|9
3972
6V
VM
EL
FAD
VT
PR
WS
Rib
osom
alpr
otei
nL
1211
219
gi|3
9866
95V
TG
GE
VG
AA
SSL
AP
K,
VSV
VP
SAA
ALV
IK
WS
Cyc
loph
ilin
566
gi|9
3972
6V
VM
EL
FAD
VT
PR
WS
Cyc
loph
ilin
538
gi|8
2911
9V
FF
DM
TIG
GQ
PAG
R
WS
His
tone
H2B
.145
9gi
|122
02A
MSI
MN
SFIN
DIF
EK
15C
ontr
ol79
2(+2
)–
MS/
MS,
Cal
mod
ulin
-bin
ding
prot
ein
60-A
(Fra
gmen
t)
12
34
56
7676
**Q
8H6U
0E
LVA
NE
DM
QH
LL
R**
*
Con
trol
842(
+2)
–M
S/M
SN
TV
DD
GSP
LL
LSS
PL
R**
*
WS
60S
ribo
som
alpr
otei
nL
23a
(L25
)62
11gi
|585
876
LTP
DY
DA
LD
VA
NK
IGII
WS
792(
+2)
–M
S/M
S,C
alm
odul
in-b
indi
ngpr
otei
n60
-A(F
ragm
ent)
ELV
AN
ED
FQ
HL
LR
***
16C
ontr
ol88
7(+2
)–
MS/
MS,
Nuc
leos
ide
diph
osph
ate
kina
seI
(EC
2.7.
4.6)
(ND
KI)
12
34
56
5062
**P
4792
2Q
NQ
TF
LM
LQ
***
WS
Pep
tide
887
m/z
Physiology and proteomics of the water-deficit stress response 393
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
Tab
le3.
Con
tinue
d
Ban
dN
o.Tr
eatm
ent
Pro
tein
iden
tifie
dR
elat
ive
abun
danc
e1
23
45
6Sc
ore
Sequ
ence
cove
rage
Acc
essi
onP
epti
de
17C
ontr
olL
ipox
ygen
ase
(EC
1.13
.11.
12)
3–
soyb
ean
12
34
56
742
gi|8
1793
LVIE
DY
PY
AV
DG
LE
IWD
AIK
WS
1122
(+2)
–M
S/M
S,G
lyci
nede
hydr
ogen
ase
[dec
arbo
xyla
ting
],m
itoc
hond
rial
prec
urso
r(E
C1.
4.4.
2)
6790
**P
2696
9F
DE
TT
SLE
DV
HA
VT
PV
***
22C
ontr
ol75
1(+2
)–
MS/
MS,
Per
mea
sepr
otei
nof
suga
rA
BC
tran
spor
ter*
12
34
56
6690
**Q
98JY
6E
YN
LL
PD
HLV
G**
*
WS
Rib
ulos
e-ph
osph
ate
3-ep
imer
ase,
chlo
ropl
ast
prec
urso
r(P
ento
se-5
-ph
osph
ate
3-ep
imer
ase)
(PP
E)
(RP
E)
(P5P
3E)
545
gi|2
4997
28SD
IIV
SPSI
LSA
NF
SK
WS
646(
+2)
–M
S/M
S,C
hlor
ophy
lla/
b-bi
ndin
gpr
otei
nty
peII
I(F
ragm
ent)
7472
**Q
9M53
8W
LA
YG
EL
LD
GR
***
WS
729(
+2)
–M
S/M
S,C
arbo
nic
anhy
dras
eN
VA
NLV
PPA
AL
NH
E**
*
23C
ontr
olC
yclo
phili
n
12
34
56
576
gi|9
3972
6V
VM
EL
FAD
VT
PR
WS
Cyc
loph
ilin
386
gi|9
3972
6V
VM
EL
FAD
VT
PR
Rel
ativ
eab
unda
nce
ofse
lect
edpr
otei
nsis
show
nas
aba
rgr
aph:
lane
1,C
OC
041
wel
lwat
ered
;lan
e2,
CO
C04
1w
ater
stre
ssed
;lan
e3,
CO
C16
6w
ellw
ater
ed;l
ane
4,C
OC
166
wat
erst
ress
ed;l
ane
5,T
MV
2w
ellw
ater
ed;l
ane
6,T
MV
2w
ater
stre
ssed
.W
S,w
ater
stre
ss;@
,pro
tein
sid
enti
fied
byon
e-di
men
sion
al(1
-D)
shot
gun
ofth
eex
cise
dba
ndre
sult
ing
inm
ulti
ple
hits
,but
scor
ean
dac
cess
ion
num
ber
ofth
efir
sthi
tfo
rea
chpr
otei
nw
ere
men
tion
edin
the
tabl
e,an
dpe
ptid
ese
quen
ces
ofal
lhit
sar
epr
ovid
edin
Supp
orti
ngIn
form
atio
nTa
ble
S2.
*,es
tim
ated
sequ
ence
;**,
prot
ein
iden
tity
;***
,de
novo
sequ
ence
.D
iffe
renc
esbe
twee
nth
etr
eatm
ents
wer
esi
gnifi
cant
atP
<0.
0001
.
394 K. R. Kottapalli et al.
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
1 2 3 4 5 67 89 10
111213 14
15
16 17
1819 20
21
22
23 24
25 26
2728
M (kDa) M (kDa)7 4
250150100
75
50
37
25
20
15
10
407
509 COC 041 – Water stress
COC 041 – Control
1 2 3 4 5 67 89 10
111213 14
15
16 17
1819 20
21
22
23 24
25 26
27
12–1
4% S
DS–
PA
GE
IPG (18 cm)
(a) (b)
28
COC 166 – Waterstress
29 30
31 32
33
59
58
43
3536
40
37 38
3941
4244 53
45
46
5047 4849
5152
54 5556
57
34
7 4
250150
100
75
50
37
25
20
15
10
446
491 C
COC 166 – Control
29 30
31 32
33
59
58
43
3536
40
37 38
3941
4244 53
45
46
5047 4849
5152
54 5556
57
12–1
4% S
DS–
PA
GE
34
IPG (18 cm)
7
60 61
78
64
6779
62 63
7571
76 77
65
6968
66
74
73
70
71
72
M (kDa)7 4
250150100
75
50
37
2520
15
10
375 TMV 2 – Control
7
60 61
365 TMV 2 – Water stress
78
64
6779
62 63
7571
76 77
65
6968
66
74
73
70
71
72
12–1
4% S
DS–
PA
GE
IPG (18 cm)
(c)
Figure 5. Two-dimensional gel electrophoresis (2-DGE) leafprotein profiles of three peanut genotypes. (a) Mini-coregenotype COC041 control and water stressed. (b) Mini-coregenotype COC166 control and water stressed. (c) Moderatelystress-tolerant cultivar TMV2 control and water stressed. Leafproteins (80 mg) were separated on 18 cm IPG (pH 4.0–7.0)strips in the first dimension followed by sodium dodecylsulphate–polyacrylamide gel electrophoresis (SDS–PAGE) ongradient (12–14%) large-format gels in the second dimension.Proteins were stained with silver nitrate. Five microlitres of themolecular mass standards (Bio-Rad) was loaded adjacent to theacidic end of the IPG strip. Image analysis detected 407, 509, 446,491, 375 and 365 spots on the two-dimensional (2-D) gels, forCOC041, COC166 and TMV2 control and water-stressedsamples, respectively. Numbered arrows, boxes or circles (spots1–79) show stress-responsive proteins. Blue indicates proteinsabundant under control conditions, but decreased or absentfollowing water stress, and red indicates proteins increasedfollowing water stress. The positions of the proteins are markedin the same direction and position for clarity, in each of the gels.
Physiology and proteomics of the water-deficit stress response 395
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
oxygen production induced by water-deficit stress (Osmond& Grace 1995; Kozaki & Takeba 1996; Noctor et al. 2002).
Acetyl CoA carboxylase (ACC) mediated cellwall strengthening under water stress
Interestingly, ACC (Table 4, spots 26 and 27), which is anenzyme involved in lipid biosynthesis, was uniquely identi-fied in the tolerant genotype (COC041) and detectable onlyduring water stress. In plants, ACC isozymes provide themalonyl CoA pools used for de novo fatty acid synthesis inplastids and mitochondria, and for fatty acid elongation,flavonoid (FL) and stilbene biosynthesis in the cytosol(Focke et al. 2003). From several studies, it is evident thatthe ACC reaction is the most important regulatory step,controlling metabolite flow in response to stress. From thewater-deficit stress tolerance perspective, fatty acids areessential in membrane biogenesis, lipoic acid and cuticularwax synthesis and stress signalling (Zuther et al. 2004).Under extreme water deficit when stomata are nearly com-pletely closed, water loss is primarily through cuticular tran-spiration (Shepherd & Griffiths 2006). In response to waterstress, epicuticular wax deposition is initiated within a fewdays (Premachandra et al. 1991), and tolerant plants oftenhave thicker leaf wax than susceptible plants (Shepherd &Griffiths 2006). To test this hypothesis, we measured theEWL in both well-watered and water-stressed plants. Inter-estingly, there was significantly higher EWL in the tolerantgenotype (COC041) compared to the susceptible genotype(COC166) under normal conditons. Although EWL wasslightly increased in the tolerant genotype during stress,there was a significant decrease in EWL in the susceptiblegenotype (COC166) (Fig. 7). In alfalfa, transgenic plantswith increased cuticular waxes showed reduced water lossand decreased chlorophyll leaching, thereby enhancingtolerance to water-deficit stress (Zhang et al. 2005). Theseresults support our hypothesis that a higher level of ACCprotein in tolerant peanut leaves leads to increasedamounts of polyunsaturated fatty acids, thicker cuticularwax and flavonoids for water-deficit stress signalling.
Reduction in photosynthesis-related proteinsduring water stress in tolerant genotypes
Nine differentially accumulated protein spots (Table 4,spots 12, 13, 14, 23, 34, 62, 63, 68, 74) were identified asRubisco large subunit (LSU) or small subunit (SSU).1-DGE and Western blot with Rubisco LSU indicated ageneral reduction in Rubisco protein content in bothtolerant (COC041) and susceptible (COC166) genotypes(Fig. 4). However, the protein was increased in the moder-ately tolerant cultivar (TMV2) during water stress. 2-Danalysis revealed five spots (12, 13, 14, 68, 74) identified asfractions of Rubisco protein that were also reduced in theleaves of the tolerant genotypes (COC041 and TMV2). Car-bonic anhydrase (CA) (Table 3, bands 1 and 3) and oxygenevolving enhancer protein 2 (OEP) of photosystem II(PSII) were also reduced in the tolerant genotype
(COC041). Interestingly, another nuclear-encoded PSIIprotein, psbP (Table 4, spot 73), decreased only in the tol-erant genotype. The abundance of two protein bands iden-tified as photosynthesis-related chlorophyll a/b-bindingprotein (Table 3, bands 11 and 22) also declined in the tol-erant genotype, but its homolog (Table 4, spot 71) wasinduced during water-deficit stress. Together, these resultssuggest an overall reduction of photosynthesis-related pro-teins during water stress in the tolerant peanut genotypes.Correlated with this decrease in major photosynthetic pro-teins was a rapid decrease in transpiration and photosyth-etic rate in the tolerant genotype compared to susceptibleplants (Table 2; Fig. 3).
Increased ATP synthase and ferredoxin–NADPreductase to meet energy demand duringwater stress
Because water stress substantially decreases CO2 assimila-tion by net reduction in the amount of ATP (Tezara et al.1999), it was suggested that induction of ATP synthesis willassist in abiotic stress tolerance (Zhang, Liu & Takano2008). In the current study, an ATP synthase epsilon chain(Table 4, spot 28) and an ATP synthase beta subunit(Table 3, band 2A) were highly induced only in tolerantgenotypes suggesting their putative role in water-stress tol-erance. ATP synthase plays a central role in energy trans-duction in chloroplasts and mitochondria, and alleviationof stress. The protein was reported to be induced in salt-stressed rice leaves (Kim et al. 2005) and shoots and rootsof maize (Zörb et al. 2004). Over-expression of the ATPsynthase gene resulted in greater tolerance to drought inArabidopsis (Zhang et al. 2008). Induction of the protein intolerant peanut genotypes may alleviate water-deficit stressby increasing ATP supply to meet increased stress-relatedenergy demand. In addition, ferredoxin–NADP reductasewhich is involved in electron transfer, was also induced in allthe genotypes and may help in meeting the energy demandduring stress.
Lectin and lactoglutathione lyase proteins aswater-deficit stress markers
Several lectins including galactose-binding and mannose/glucose-binding isoforms (bands 7, 10, and spots 17, 18, 36,38–50, 60 and 61) were highly induced in the susceptiblegenotype. By contrast, lectin proteins remained eitherunchanged or undetectable in the tolerant COC041 andTMV2 genotypes.While the role of lectins in the plant stressresponse is not clear, several studies have shown inductionof specific lectins in response to both abiotic and bioticstresses, and provided some evidence for lectins in diversefunctions from cell wall modification to regulation of geneexpression (Van Damme et al. 2004; Bhushan et al. 2007;Aghaei et al. 2008; Jia et al. 2008). Bhushan et al. (2007)reported induction of a mannose lectin (gi6822274)in stress-tolerant chickpea only during water-deficit stress.
396 K. R. Kottapalli et al.
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
Tab
le4.
Lis
tof
wat
erst
ress
-res
pons
ive
leaf
prot
ein
spot
sfr
omtw
o-di
men
sion
alge
lele
ctro
phor
esis
(2-D
GE
)id
enti
fied
bym
ass
spec
trom
etry
(MS)
Spot
No.
Pro
tein
iden
tifie
dR
elat
ive
abun
danc
eA
cces
sion
MW
/pI
Scor
eSe
quen
ceco
vera
geM
SP
epti
de
1M
ethi
onin
esy
ntha
se[G
lyci
nem
ax]
EC
1.16
.1.8
12
34
56
gi|3
3325
957
8440
1/5.
9310
34
Q-T
OF
YG
WT
GG
EIG
FD
TY
FSM
AR
/TLT
SLN
GV
TA
YG
FD
LVR
2H
SP70
-3(s
ame
spot
s=
3an
d4)
12
34
56
gi|1
5232
682
7155
9/4.
9790
23M
AL
DI
TT
PSY
VA
FT
DSE
R/E
FSA
EE
ISSM
ILIK
MR
/NA
VV
TV
PAY
FN
DSQ
R/D
AG
VIA
GL
NV
MR
/DA
GV
IAG
LN
VM
R/I
INE
PT
AA
AIA
YG
LD
K/I
INE
PT
AA
AIA
YG
LD
KK
/MV
NH
FV
QE
FK
R/F
EE
LN
IDL
FR
/DN
NL
LG
KF
EL
SGIP
PAP
R/F
EL
SGIP
PAP
R/N
AL
EN
YA
YN
MR
/MY
QG
GE
AG
GPA
AG
GM
DE
DV
PP
SAG
GA
GP
K
5H
eat
shoc
kpr
otei
n70
prec
urso
r[C
itrul
lus
lana
tus]
(sam
esp
ots
=6–
8)1
23
45
6
gi|1
9289
9175
656/
5.70
7820
MA
LD
IQ
FAA
EE
ISA
QV
LR
/QFA
AE
EIS
AQ
VL
RK
/AV
VT
VPA
YF
ND
SQR
/IIN
EP
TA
ASL
AY
GF
EK
/IIN
EP
TA
ASL
AY
GF
EK
K/A
KM
EL
SSLT
QA
NIS
LP
FIT
AT
AD
GP
K/F
EE
LC
SDL
LYR
/FE
EL
CSD
LLY
RL
K/D
VH
EV
VLV
GG
STR
IPA
VQ
ELV
K/S
EV
FST
AA
DG
QT
SVE
INV
LQ
GE
R/S
LG
SFR
LD
GIP
PAP
R
12R
ibul
ose
1·5-
bisp
hosp
hate
carb
oxyl
ase-
oxyg
enas
ela
rge
subu
nit[
Dal
embe
rtia
popu
lifol
ia]
12
34
56
gi|6
2861
135
5186
2/6.
3024
943
MA
LD
ILT
YY
TP
EY
ET
K/L
TY
YT
PE
YE
TK
DT
DIL
AA
FR
/DT
DIL
AA
FR
/AL
RL
ED
LR
/LE
DL
RIP
ISY
IK/I
PI
SYIK
TF
QG
PP
HG
IQV
ER
/TF
QG
PP
HG
IQV
ER
/YG
RP
LL
GC
TIK
PK
/GG
LD
FT
KD
DE
NV
NSQ
PF
MR
/GG
LD
FT
KD
DE
NV
NSQ
PF
MR
/DR
FL
FC
AE
AIF
K/F
LF
CA
EA
IFK
/GH
YL
NA
TA
GT
CE
EM
IKR
/D
NG
LL
LH
IHR
/QK
NH
GM
HF
R/Q
KN
HG
MH
FR
/L
SGG
DH
IHA
GT
VV
GK
/LE
GE
RD
ITL
GF
VD
LL
R/D
ITL
GF
VD
LL
R/D
ITL
GF
VD
LL
RD
DF
IEK
/VA
LE
AC
VQ
AR
/WSP
EL
AA
AC
EV
WK
/AIK
FE
FP
AM
DT
L/A
IKF
EF
PAM
DT
L
13C
hlor
opla
stri
bulo
se1·
5-bi
spho
spha
teca
rbox
ylas
e/ox
ygen
ase
acti
vase
smal
lpr
otei
nis
ofor
m[A
cer
rubr
um]
12
34
56
gi|1
1533
4979
4795
2/7.
5775
31M
AL
DI
NF
MSL
PN
IKIP
LIL
GIW
GG
K/S
FQ
CE
LVFA
K/M
GIT
PIM
MSA
GE
LE
SGN
AG
EPA
KL
IR/M
CC
LF
IN
DL
DA
GA
GR
/MC
CL
FIN
DL
DA
GA
GR
/FY
WA
PT
R/F
YW
AP
TR
ED
R/L
VD
TF
PG
QSI
DF
FG
AL
R/
LL
EY
GN
MLV
QE
QE
NV
K/L
LE
YG
NM
LVQ
EQ
EN
VK
R/V
QL
AD
KY
LSE
AA
LG
DA
ND
DA
IK
14C
hlor
opla
stri
bulo
se1·
5-bi
spho
spha
teca
rbox
ylas
e/ox
ygen
ase
acti
vase
smal
lpr
otei
nis
ofor
m[A
cer
rubr
um]
12
34
56
gi|1
1533
4979
4795
2/7.
5758
15M
AL
DI
SFQ
CE
LVFA
K/M
CC
LF
IND
LD
AG
AG
R/M
CC
LF
IND
LD
AG
AG
R/F
YW
AP
TR
ED
R/L
VD
TF
PG
QSI
DF
FG
AL
R/L
LE
YG
NM
LVQ
EQ
EN
VK
R
Physiology and proteomics of the water-deficit stress response 397
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
Tab
le4.
Con
tinue
d
Spot
No.
Pro
tein
iden
tifie
dR
elat
ive
abun
danc
eA
cces
sion
MW
/pI
Scor
eSe
quen
ceco
vera
geM
SP
epti
de
16Fe
rred
oxin
–NA
DP
redu
ctas
e,le
afis
ozym
e,ch
loro
plas
tpr
ecur
sor
(FN
R)
EC
1.18
.1.2
12
34
56
gi|1
1990
540
454/
8.56
544
Q-T
OF
LYSI
ASS
AIG
DF
GD
SK
17L
ecti
n(s
ame
spot
s=
18an
d44
–48)
12
34
56
P93
536
E*
E*
Q-T
OF
NL
LL
QG
DA
HL
DP
NV
LQ
LTR
/VL
AV
EM
DT
FM
DR
/LQ
GD
AH
LD
PN
DP
QLT
R
21A
ldol
ase
(sam
esp
ots
=33
and
79)
EC
4.1.
2.13
12
34
56
gi|1
6903
937
974/
5.47
628
Q-T
OF
YA
AIS
QD
NG
LVP
IVE
PE
ILL
DG
EH
GID
R
23R
ibul
ose
1·5-
bisp
hosp
hate
carb
oxyl
ase/
oxyg
enas
ela
rge
subu
nit
[For
chha
mm
eria
palli
da]
12
34
56
gi|4
6325
921
3867
6/6.
6877
17M
AL
DI
LTY
YT
PE
YE
TK
DT
DIL
AA
FR
/DT
DIL
AA
FR
/A
LR
LE
DL
R/T
FQ
GP
PH
GIQ
VE
R/A
VR
LSG
GD
HV
HA
GT
VV
GK
25C
rist
al-G
lass
1pr
otei
n[C
apsi
cum
annu
um]
12
34
56
gi|4
0287
530
2060
7/6.
8274
32M
AL
DI
SPG
YY
DG
R/S
PG
YY
DG
RY
WT
MW
K/Y
WT
MW
K/L
PM
FG
CT
DA
TQ
VL
NE
VQ
EA
K/L
PM
FG
CT
DA
TQ
VL
NE
VQ
EA
K/L
PM
FG
CT
DA
TQ
VL
NE
VQ
EA
KK
/IIG
FD
NV
R/Q
VQ
CIS
FIA
YK
PE
GY
26A
cety
l-C
oAca
rbox
ylas
eca
rbox
yltr
ansf
eras
ebe
tasu
buni
t[E
ucal
yptu
sgl
obul
ussu
bsp.
glob
ulus
](s
ame
spot
=27
)E
C6.
4.1.
2
12
34
56
gi|1
0880
2652
5604
2/5.
6071
10M
AL
DI
ME
KW
WF
NSM
LYK
/WW
FN
SMLY
KG
K/N
FI
SDD
TF
LVR
/KT
GLT
DA
VQ
TG
TG
R/G
LF
DP
IVP
RN
PL
K
398 K. R. Kottapalli et al.
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
28A
TP
synt
hase
epsi
lon
chai
n(A
TP
synt
hase
F1
sect
orep
silo
nsu
buni
t)E
C3.
6.3.
14
12
34
56
gi|1
1459
814
654/
5.84
4812
Q-T
OF
LN
DQ
WV
TM
AL
MG
GFA
R
301l
-myo
-ino
sito
l-1-
phos
phat
esy
ntha
se[P
hase
olus
vulg
aris
]E
C5.
5.1.
4
12
34
56
gi|1
4582
467
5243
5/5.
4437
2Q
-TO
FV
GSY
QG
EE
IYA
PF
K
34R
ibul
ose
1·5-
bisp
hosp
hate
carb
oxyl
ase/
oxyg
enas
esm
all
subu
nit
[Aeg
ilops
taus
chii]
12
34
56
gi|4
0387
1118
770/
8.83
7942
MA
LD
IV
MA
SSA
TT
VA
PF
QG
LK
/VM
ASS
AT
TV
AP
FQ
GL
KST
AG
LP
VSR
/IR
CM
QV
WP
IEG
IK/F
ET
LS
YL
PP
LST
EA
LL
K/W
VP
CL
EF
SKV
GIV
FR
35P
utat
ive
lact
oylg
luta
thio
nely
ase
(Met
hylg
lyox
alas
e)(A
ldok
etom
utas
e)(G
lyox
alas
eI)
(Glx
I)(K
eton
e-al
dehy
dem
utas
e)E
C4.
4.1.
5
12
34
56
gi|2
4948
4331
740/
5.19
103
8Q
-TO
FD
PD
GY
TF
EL
IQR
/IV
SFL
DP
DG
WK
36G
alac
tose
-bin
ding
lect
inpr
ecur
sor
[Ara
chis
hypo
gaea
](s
ame
spot
=38
)1
23
45
6
AA
A74
571
26.6
71**
Q-T
OF
NG
DLT
TL
AD
VV
EL
K
37R
etro
tran
spos
onpr
otei
n,pu
tati
ve,u
ncla
ssifi
ed[O
ryza
sativ
a(j
apon
ica
cult
ivar
-gro
up)]
12
34
56
gi|7
7553
936
8406
0/6.
1069
14M
AL
DI
AE
VE
PV
NV
IPV
AL
EE
LD
EG
AR
/AY
TQ
DL
LM
KA
CA
R/M
MV
PK
NP
EV
GV
WK
/SN
AG
TSS
SQA
AG
LTR
PSG
R/F
NE
LR
PL
PT
KM
WR
/HK
SIE
IEE
PV
VV
QK
/ST
KN
DIS
ET
IED
FD
EV
EK
39C
hain
A,c
ryst
alst
ruct
ure
ofdi
ocle
avi
olac
ease
edle
ctin
(sam
esp
ots
=40
–43,
60an
d61
)1
23
45
6
2GD
F_A
27.3
66*
Q-T
OF
TSD
LG
DP
NY
PH
LG
LD
YF
47F
lava
none
3-hy
drox
ylas
e[C
itrus
sine
nsis
]E
C1.
14.1
1.9
12
34
56
gi|4
1264
0140
815/
5.99
6936
MA
LD
IM
AP
STLT
AL
AG
EK
TL
NP
SFV
R/A
PST
LTA
LA
GE
K/T
LN
PSF
VR
FQ
DE
RP
K/V
AY
NE
FSN
EIP
VIS
LA
GID
DV
GG
KR
/LIS
DM
TR
LA
TE
FFA
LP
PE
EK
/GG
FIV
SSH
LQ
GE
VV
K/W
PD
KP
EG
WM
EV
TK
EY
SDK
/HT
DP
GT
ITL
LL
QD
QV
GG
LQ
AT
KD
NG
K
Physiology and proteomics of the water-deficit stress response 399
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
Tab
le4.
Con
tinue
d
Spot
No.
Pro
tein
iden
tifie
dR
elat
ive
abun
danc
eA
cces
sion
MW
/pI
Scor
eSe
quen
ceco
vera
geM
SP
epti
de
49M
anno
se/g
luco
se-b
indi
ngle
ctin
prec
urso
r[A
rach
ishy
poga
ea]
12
34
56
gi|9
5111
828
372/
5.36
5710
Q-T
OF
LD
SLSF
SYN
NF
EQ
DD
ER
NL
ILQ
GD
AK
50M
anno
se/g
luco
se-b
indi
ngle
ctin
prec
urso
r[A
rach
ishy
poga
ea]
(sam
esp
ots
=51
and
52)
12
34
56
gi|9
5111
030
994/
5.71
738
Q-T
OF
SPID
NG
AD
GIA
FF
IAA
PD
SEIP
K
62R
ibul
ose
1·5-
bisp
hosp
hate
carb
oxyl
ase-
oxyg
enas
ela
rge
subu
nit
[Ara
chis
hypo
gaea
]
12
34
56
gi|2
3428
8451
949/
6.19
208
40M
AL
DI
LTY
YT
PE
YE
TK
/LT
YY
TP
EY
ET
KD
TD
ILA
AF
R/D
TD
ILA
AF
R/A
LR
LE
DL
R/L
ED
LR
IPIS
YIK
/T
FQ
GP
PH
GIQ
VE
R/T
FQ
GP
PH
GIQ
VE
RD
K/Y
GR
PL
LG
CT
IKP
K/A
VY
EC
LR
/GG
LD
FT
KD
DE
NV
NSQ
PF
MR
/GG
LD
FT
KD
DE
NV
NSQ
PF
MR
/D
RF
LF
CA
EA
IFK
/GH
YL
NA
TA
GT
CE
EM
IKR
/D
NG
LL
LH
IHR
/QK
NH
GM
HF
R/L
SGG
DH
IHA
GT
VV
GK
/VA
LE
AC
VQ
AR
/EG
NE
IIR
EA
SK/E
ASK
WSP
EL
AA
AC
EV
WK
/WSP
EL
AA
AC
EV
WK
63R
ibul
ose
1·5-
bisp
hosp
hate
carb
oxyl
ase-
oxyg
enas
ela
rge
subu
nit
[Ara
chis
hypo
gaea
]
12
34
56
gi|2
3428
8451
949/
6.19
178
36M
AL
DI
LTY
YT
PE
YE
TK
DT
DIL
AA
FR
/DT
DIL
AA
FR
/AL
RL
ED
LR
/LE
DL
RIP
ISY
IK/T
FQ
GP
PH
GIQ
VE
R/T
FQ
GP
PH
GIQ
VE
RD
K/Y
GR
PL
LG
CT
IKP
K/
YG
RP
LL
GC
TIK
PK
/AV
YE
CL
R/G
GL
DF
TK
DD
EN
VN
SQP
FM
R/G
GL
DF
TK
DD
EN
VN
SQP
FM
R/D
NG
LL
LH
IHR
/QK
NH
GM
HF
R/L
SGG
DH
IHA
GT
VV
GK
/VA
LE
AC
VQ
AR
/EG
NE
IIR
EA
SK/E
ASK
WSP
EL
AA
AC
EV
WK
/WSP
EL
AA
AC
EV
WK
/AIK
FE
FPA
MD
TL
/AIK
FE
FPA
MD
TL
67P
last
idic
aldo
lase
NPA
LD
P1
[Nic
otia
napa
nicu
lata
]
12
34
56
gi|4
8272
5142
832/
6.92
7926
MA
LD
IG
ILA
MD
ESN
AT
CG
KR
/GIL
AM
DE
SNA
TC
GK
R/R
LA
SIG
LE
NT
EA
NR
/LA
SIG
LE
NT
EA
NR
/LA
SIG
LE
NT
EA
NR
QA
YR
/VD
KG
LVP
LA
GSN
DE
SWC
QG
LD
GL
ASR
/GLV
PL
AG
SND
ESW
CQ
GL
DG
LA
SR/S
AA
YY
GA
R/W
RT
VV
SIP
NG
PS
AL
AV
K/T
WG
GR
PE
NV
QA
AQ
EA
LL
IR
400 K. R. Kottapalli et al.
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
68R
ibul
ose-
bisp
hosp
hate
carb
oxyl
ase
acti
vase
(EC
6.3.
4.-)
Alo
ngfo
rmpr
ecur
sor
–ba
rley
(fra
gmen
t)(s
ame
spot
=69
)
12
34
56
gi|1
0061
447
496/
5.64
253
Q-T
OF
IVD
TF
PG
QSI
DF
FG
AL
R
71P
utat
ive
chlo
roph
yll
a/b-
bind
ing
prot
ein
[Fag
ussy
lvat
ica]
12
34
56
gi|7
3665
920
2768
5/5.
1465
12M
AL
DI
NV
SSG
SPW
YG
PD
R/N
VSS
GSP
WY
GP
DR
VK
/NR
EL
EV
IHSR
/FG
EA
VW
FK
73P
sbP
[Xer
ophy
tahu
mili
s]
12
34
56
gi|2
5992
740
2634
7/6.
8463
5Q
-TO
FT
NT
DF
LTY
AG
DG
FK
74R
ibul
ose
1·5-
biph
osph
ate
carb
oxyl
asel
/oxy
gena
sela
rge
subu
nit
12
34
56
AB
M63
291
28.5
100*
*Q
-TO
FLT
YY
TP
EY
ET
K
78F
OG
:TP
Rre
peat
(ISS
)[O
stre
ococ
cus
taur
i]
12
34
56
gi|1
1600
0496
7251
8/5.
0968
10M
AL
DI
NA
GM
PSG
EIA
AF
TK
K/Y
QK
AQ
EL
AL
R/A
LA
SDP
SDE
TV
R/Y
SDLV
NA
IKSE
FG
IEK
/MD
LR
TA
LTN
FAA
VA
ER
Rel
ativ
eab
unda
nce
ofse
lect
edpr
otei
nsis
show
nas
aba
rgr
aph:
lane
1,C
OC
041
wel
lwat
ered
;lan
e2,
CO
C04
1w
ater
stre
ssed
;lan
e3,
CO
C16
6w
ellw
ater
ed;l
ane
4,C
OC
166
wat
erst
ress
ed;l
ane
5,T
MV
2w
ellw
ater
ed;l
ane
6,T
MV
2w
ater
stre
ssed
.*,
esti
mat
edse
quen
ce;*
*,pr
otei
nid
enti
ty.
Dif
fere
nces
betw
een
the
trea
tmen
tsw
ere
sign
ifica
ntat
P<
0.00
01.
MA
LD
I,m
atri
x-as
sist
edla
ser
deso
rpti
on/io
niza
tion
;Q-T
OF,
quad
rupo
leti
me-
of-fl
ight
.
Physiology and proteomics of the water-deficit stress response 401
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
Interestingly, lectin expression appears to be unaffectedin the tolerant genotypes (COC041 and TMV2), whileinduced in the susceptible COC166 plants in response towater-deficit stress. Aghaei et al. (2008) reported a similardown-regulation of lectins in response to salt stress insoybean hypocotyls and roots. Immunoblotting studies witha rice polyclonal anti-SalT antibody revealed that the saltand water stress-inducible mannose lectin protein SalT(Claes et al. 1990; Kim et al. 2005) was also induced in thesusceptible COC166 plants during stress (Fig. 8). However,in tolerant genotypes (COC041 and TMV2), the SalTprotein disappeared after stress. A greater induction oflectins in COC166 could indicate that this genotype expe-rienced severe water stress. On the contrary, tolerant geno-types might not have experienced water stress because ofthe presence of other compensatory mechanisms; therefore,increased abundance of SalT was not evident under water-deficit conditions. There was also a significant inductionof lactoglutathione lyase (Table 4, spot 35), the proteininvolved in glyoxalase system, in the susceptible COC166
plants in response to water deficit, while the protein wasundetectable in the tolerant genotypes. Lactoglutathionelyase is one of the two enzymes of the glyoxalase systemassociated with detoxification of cytotoxic methylglyoxal,formed as a by-product of carbohydrate and lipid metabo-lism (Thornalley 1993). The absence of this protein in thetolerant genotype (COC041) and induction in susceptibleaccession, as well as the contrasting amount of detectablelectins, indirectly points to the general status of cells instress-tolerant and susceptible genotypes during water-deficit stress.
Histone H2B and retrotransposon-based novelgene regulation under water-deficit stress
A histone H2B protein was induced in the susceptible line,and the retrotransposon protein (Table 4, spot 37) appearedin the tolerant genotype (COC041) during water stress. Inyeast, it was shown that histone H2B, upon ubiquitination,regulates histone H3 methylation and transcriptionalsilencing (Sun & Allis 2002). Such unique gene regulationmediated through ‘trans-tail’ histone modification cannotbe ruled out during water stress in peanuts. However, theexact mechanism of water-deficit stress tolerance involvingreduction of histone proteins in the TMV2 cultivar remainsenigmatic. It is known that retrotransposons can generatesmall RNAs (siRNA) which in turn may silence a specificgene (Watanabe et al. 2006). Currently, we do not know ifthe identified retrotransposon in tolerant peanut genotypesgenerates siRNA, which can knock down a gene whoseproduct is detrimental to the cells during water stress.
Transcript response to water-deficit stress
To investigate whether changes in gene expression werecorrelated to changes in protein abundance, a qRT-PCRexperiment was conducted using the available ESTsequences of eight candidate proteins (Fig. 9). Not surpris-ingly, these results showed that in most instances, the
Photosynthesis25%
Photorespiration2%
Drought/Stressresponsive
10%
Lipid biosynthesis2%
Signalling proteins13%
Lectins15%
Energy metabolism8%
Detoxifying enzymes2%
Miscellaneous/Unknown17%
Novel gene regulation4%
Flavonoid pathway2%
Figure 6. Functional categorization of proteins detected fromboth one-dimensional (1-D) and two-dimensional (2-D) gels andidentified by tandem mass spectrometry (MS/MS),matrix-assisted laser desorption/ionization (MALDI) andquadrupole time-of-flight (Q-TOF) analyses.
0
1
2
3
4
5
6
COC166 COC041
Epi
cuti
cula
r w
ax lo
ad(m
g w
ax d
m–2
)
Water-deficit stressWell watered
*
Figure 7. Leaf epicuticular wax load (EWL) of susceptible (COC166) and tolerant (COC041) peanut genotypes for water-deficitstressed leaves (black bars) 7 d post-irrigation and well-watered control plants (white bars). Bars represent mean values � SE. Statisticallysignificant differences are indicated as *P = 0.0006.
402 K. R. Kottapalli et al.
© 2009 Blackwell Publishing Ltd, Plant, Cell and Environment, 32, 380–407
mRNA levels did not correlate with protein abundance.Methionine synthase protein levels declined in all geno-types in response to water-deficit stress and were correlatedwith a decrease in transcript levels in TMV2 and COC166(Fig. 9). However, the transcript for this gene nearlydoubled in stressed COC041 leaves. Lectin mRNA in toler-ant COC041 and methionine synthase, and TPR transcripts
in TMV2 correlated with respective protein patterns. Inthe susceptible genotype (COC166), four transcripts (i.e.methionine synthase, NDK1, 1l-myo-inositol-1-phosphatesynthase and TPR expression patterns) were well corre-lated with protein patterns. Several studies reported similarfindings regarding changes at the transcript level which donot correlate with changes in total protein because of post-translational regulation of gene expression (Hirano et al.2007; Joosen et al. 2007; Kottapalli et al. 2007b).
Theoretical model of water stress tolerancein peanuts
Based upon our results, we developed a theoretical modelrepresenting water stress tolerance in peanuts (Fig. 10).Peanut, an oilseed crop, might be utilizing its ability toadjust the lipid composition in addition to increased pro-duction of downstream metabolites (e.g. jasmonates) toreduce the impact of water stress. Initially, the perception ofwater stress apparently induced the production of signallingproteins, including CBP, cyclophilin, NDK1 and aldolases.Subsequently, leaves modified cell walls through lignifica-tion and wax deposition to minimize water loss. MalonylCoA pools may also generate jasmonates through theaction of lipoxygenases, which participate in long-distancesignalling. Defence-related proteins (e.g. lectins and redoxproteins) may be induced at a later stage. Finally, as a con-sequence of water stress, the photosynthetic machinerymay be reversibly and partially de-activated to reduce det-rimental loss of water, but may be rapidly activated upon
Anti-SalT (rice polyclonal)
1
15 mg protein
2 3 4 5 6M
25
20
15
Figure 8. One-dimensional (1-D) immunoblotting showingcross-reacting SalT protein in peanut leaves. Leaves from controland water-stressed plants were sampled at 7 d post-treatment.Protein samples from COC041 control (1), COC041 water stresstreated (2), COC166 control (3), COC166 water stress treated(4), TMV2 control (5), TMV2 water stress treated (6) werementioned above each lane. Molecular weights (kDa) of proteinmarkers (Precision Plus Protein Standards, Bio-Rad) areindicated at the left. Immunoassaying was carried out asdescribed in Materials and methods.
0.00
0.25
0.50
0.75
1.00
1.25
1.50
1.75
2.00
2.25
2.50
2.75
3.00
3.25
3.50
3.75
4.00
4.25
4.50
4.75
5.00
TMV2 COC166 COC041
Lectin
LOX4
Meth Syn
Myo Inositol
NDK1
TPR
CamBP
ACC
Rel
ativ
e ex
pres
sion
of
drou
ght
resp
onsi
ve t
rans
crip
ts
Figure 9. Real-time qRT-PCR analysis using gene-specific primers for lectin, LOX, methionine synthase, myo-inositol 1-phosphate,NDK1 and TPR. The transcript level is represented as the ratio of relative gene expressions for each cultivar (ratio of water-stressed andwell-watered control). Relative quantification of gene expression was estimated by Roche E method by first normalizing the target geneto the reference actin gene followed by normalization using the calibrator (COC166 untreated) ratios.
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rewatering. This is an essential trait for production agricul-ture where plants are continually exposed to intermittentirrigation events in both rain-fed and irrigated conditions.In our tolerant genotype (COC041), a 30% decrease inirrigation levels in the field only reduced yield by 15–20%compared with 90% in the susceptible genotype, which is asubstantial difference in real-world application. This yieldresponse appears to be correlated with a rapid down-regulation of photosynthesis via stomatal closure anddecrease in photosynthetic machinery which could mini-mize water loss from the plant and prevent cellular damage.Additionally, higher epicuticular wax may minimizeadditional water loss from the tolerant genotype. Uponre-irrigation, the tolerant genotype rapidly regains a signifi-cant percentage of its non-stressed photosynthetic capacity.Interestingly, the tolerant genotypes fail to exhibit up-regulation of many proteins known to be responsive tostress, suggesting that under the similar levels of availablesoil moisture, the tolerant genotype does not experiencethe same level of stress as experienced by the susceptible
genotype. Although both tolerant and susceptible plantsrecover full photosynthetic capacity within 1 week ofre-irrigation, it is perhaps the recovery phase and potentialenergy costs associated with cellular repair that ultimatelyhave an impact on significantly reducing yield in the sus-ceptible genotype. Elucidation of the physiological mecha-nisms controlling these contrasting responses will be thefocus of our future efforts, as well as the functional charac-terization of candidate genes and proteins identified here.
ACKNOWLEDGMENTS
We thank undergraduate students, Mr Kiyotaka Horieand Ms Takako Furusawa (School of Agriculture, IbarakiUniversity, Ami, Japan), for their technical help atAIST. The anti-SalT (rice polyclonal) was donated by Prof.Kyu Young Kang, Environmental Biotechnology NationalCore Research Center, Division of Applied Life Science(BK21 program), Gyeongsang National University,Jinju 660-701, Korea. This research was supported by
Calmodulin-binding protein, cyclophilin, NDK1, aldolase, myo-inositol
Methionine synthase
DREB
nucleus
Thick cuticular wax
Calmodulin-binding protein, cyclophilin, NDK1, aldolase, myo-inositolsignalling proteins
Flavonoid9,12,15 Linolinate
Redox proteins
Water-deficit/ABA signal
Acetyl CoA carboxylaseAcetylCoA
MalonylCoA
Jasmonic acid
Lypoxygenase
Small HSPs TPR
Lignified cell walls
Lignin monomer
Methylated ligninmonomer
Methionine synthase
DREB
nucleus
Short–chain PUFA
LectinRubisco
ABA signal
Figure 10. Representative model depicting the pathways implicated in water-deficit tolerance in peanut leaves. Proteins identified in thisstudy are coloured in blue and displayed on the corresponding metabolic pathways. Solid arrows indicate induction of a particularprotein, and dashed lines represent reduction. Dark, thick arrows show the signal molecules generated downstream of a pathway. ABA,abscisic acid; NDK1, nucleoside diphosphate kinase 1; TPR, tetratricopeptide repeat; DREB, water-deficit stress response element-bindingprotein.
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grants from the National Peanut Board, Texas PeanutProducers Board, New Mexico Peanut Research Board,New Mexico State University Agricultural ExperimentStation, Ogallala Aquifer Initiative and USDA-ARS CRIS6208-21000-012-00D.
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SUPPORTING INFORMATION
Additional Supporting Information may be found in theonline version of this article:
Figure S1. Standardized protein extraction protocol frompeanut leaf using phenol buffer.Table S1. Primer list for qRT-PCR analysis of peanut genes.Table S2. Peptide sequences of all hits for the proteins iden-tified by 1-D shotgun of the excised bands 2A, 2B and 2C.
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