Skip to main content
  • Research article
  • Open access
  • Published:

Glyceraldehyde-3-phosphate dehydrogenase is largely unresponsive to low regulatory levels of hydrogen peroxide in Saccharomyces cerevisiae



The reversible oxidation of protein SH groups has been considered to be the basis of redox regulation by which changes in hydrogen peroxide (H2O2) concentrations may control protein function. Several proteins become S-glutathionylated following exposure to H2O2 in a variety of cellular systems. In yeast, when using a high initial H2O2 dose, glyceraldehyde-3-phosphate dehydrogenase (GAPDH) was identified as the major target of S-glutathionylation which leads to reversible inactivation of the enzyme. GAPDH inactivation by H2O2 functions to reroute carbohydrate flux to produce NADPH. Here we report the effect of low regulatory H2O2 doses on GAPDH activity and expression in Saccharomyces cerevisiae.


A calibrated and controlled method of H2O2 delivery - the steady-state titration - in which cells are exposed to constant, low, and known H2O2 concentrations, was used in this study. This technique, contrary to the common bolus addition, allows determining which H2O2 concentrations trigger specific biological responses. This work shows that both in exponential- and stationary-phase cells, low regulatory H2O2 concentrations induce a large upregulation of catalase, a fingerprint of the cellular oxidative stress response, but GAPDH oxidation and the ensuing activity decrease are only observed at death-inducing high H2O2 doses. GAPDH activity is constant upon incubation with sub-lethal H2O2 doses, but in stationary-phase cells there is a differential response in the expression of the three GAPDH isoenzymes: Tdh1p is strongly upregulated while Tdh2p/Tdh3p are slightly downregulated.


In yeast GAPDH activity is largely unresponsive to low to moderate H2O2 doses. This points to a scenario where (a) cellular redoxins efficiently cope with levels of GAPDH oxidation induced by a vast range of sub-lethal H2O2 concentrations, (b) inactivation of GAPDH cannot be considered a sensitive biomarker of H2O2-induced oxidation in vivo. Since GAPDH inactivation only occurs at cell death-inducing high H2O2 doses, GAPDH-dependent rerouting of carbohydrate flux is probably important merely in pathophysiological situations. This work highlights the importance of studying H2O2-induced oxidative stress using concentrations closer to the physiological for determining the importance of protein oxidation phenomena in the regulation of cellular metabolism.


The preferential and reversible oxidation of specific cysteine residues present in enzymes, transcription factors and receptors has been proposed to be the major mechanism by which oxidants may integrate into cellular signal transduction pathways [1, 2]. The sulfhydryl (SH) group of cysteine residues, especially when present in an environment that decreases its pKa, can be oxidized by hydrogen peroxide (H2O2), the main cellular reactive oxygen species. The major product of the reaction between a protein cysteinyl thiol and hydrogen peroxide is a protein sulfenic acid [3, 4] that, unless in a shielded environment, is a transient intermediate that undergoes a range of secondary reactions [1, 2]. The protein sulfenic acid can form (a) mixed disulfides with low-molecular weight thiols, mainly glutathione (S-glutathionylation), (b) intramolecular disulfides when vicinal thiols are present, (c) intermolecular disulfides between proteins or (d) reversible condensation with an adjacent amide to form a sulfenylamide. All these oxidations are reversible and, therefore, provide a mechanism by which protein function may be controlled by changes in cellular H2O2 concentration. When the levels of oxidant exposure are higher further oxidation of cysteinyl sulfenic acids can occur, leading to the formation of cysteinyl sulfinic and sulfonic acids [1, 2], which is considered largely irreversible in vivo [5]. Moreover, these higher levels of oxidative stress may often result in excessive disulfide bonding, and in the misfolding, aggregation, and degradation of proteins leading, eventually, to cell death [6, 7].

Glyceraldehyde-3-phosphate dehydrogenase (GAPDH) is a classic glycolytic enzyme that is active as a tetramer of identical 37 kDa subunits catalyzing the oxidative phosphorylation of glyceraldehyde-3-phosphate to 1,3-diphosphoglycerate by converting NAD+ to NADH. More recently, GAPDH emerged as a multifunctional protein with defined functions in numerous subcellular processes, namely a primary role in apoptosis and in a variety of critical nuclear pathways [8, 9]. In the yeast Saccharomyces cerevisiae (S. cerevisiae) three related but not identical GAPDH enzymes with different specific activities are encoded by unlinked genes designated TDH1, TDH2 and TDH3 [10]. None of the TDH genes are individually essential for cell viability, but a functional copy of either TDH2 or TDH3 is required since tdh2 Δtdh3 Δ cells are not viable [11].

Studies with mammalian cells have identified GAPDH as a target of oxidative modifications resulting in decreased activity following exposure to H2O2 [12, 13]. GAPDH has an active-site cysteine residue which, following exposure to H2O2, can be oxidized to an intramolecular disulfide and cysteic acid [14] and also undergo S-glutathionylation [13]. In S. cerevisiae growing in exponential phase, GAPDH was also identified as a major target of S-glutathionylation [15, 16] and also carbonylation [1719] and a sharp decrease in its enzymatic activity was observed [15, 16, 18, 20] following exposure to H2O2. In cell extracts exposed to H2O2 both Thdh2p and Thdh3p are S-glutathionylated, but in vivo only S-glutathionylation of Thd3p is observed [15, 16, 20].

Studies of GAPDH inactivation and S-glutathionylation in S. cerevisiae cells [1518, 20] have been performed in the exponential phase of growth using bolus additions of high doses of H2O2 that cause high levels of cell death, and so it is difficult to assess the possible regulatory role of H2O2 on GAPDH activity by inducing reversible GAPDH thiol oxidation, including S-glutathionylation. Therefore, our main aim with this study was to establish in S. cerevisiae cells at what levels, in the range of low to moderate H2O2 concentrations, is H2O2 able to cause an inhibition of GAPDH activity due to reversible and irreversible oxidation of the enzyme. To achieve this, instead of the typical H2O2 bolus addition, we exposed cells to controlled steady-state levels of H2O2, mimicking the physiological production of H2O2 in vivo. This methodology allows to study the biological effects of low to moderate levels of H2O2 [21] and by using it we were able to show that in yeast the overall GAPDH activity only decreases at high doses of H2O2. We also characterized the differential expression of the three Tdh isoenzymes when cells were exposed to H2O2 under our controlled conditions of H2O2 delivery. In stationary-phase cells Tdh1p expression emerged as a target for regulation by low H2O2 levels.


What are regulatory H2O2 concentrations?

A high enough H2O2 dose will eventually trigger the oxidation of cysteine residues, and so it is important to define whether the doses at which H2O2 is observed to inhibit GAPDH activity are either in the regulatory low range, or in the toxic high range of H2O2 concentrations.

To define what a low to moderate steady-state H2O2 dose is, the activity of catalase, an important antioxidant enzyme that removes H2O2, was measured. In exponential phase cells, catalase activity was upregulated for a 20 μM steady-state H2O2 exposure and for 40 μM H2O2 there was a two-fold increase in catalase activity (Figure 1A). As to stationary-phase, cells treated with H2O2 on the lower range of concentrations studied (50 μM) showed an increase in catalase activity (Figure 1B). This increase in catalase activity was modest when compared to that observed in exponential-phase cells, probably because catalase activity in stationary-phase cells is 15-fold higher than in exponential-phase cells, reflecting a probable higher formation of H2O2 due to mitochondrial respiration. However, for our purpose this increase in catalase activity observed at 50 μM steady-state H2O2 was sufficient to identify a range of concentrations where H2O2 triggers a regulatory response. S. cerevisiae has two catalases, peroxisomal catalase (catalase A) and cytosolic catalase (catalase T), encoded by the CTA1 and CTT1 genes respectively, and both are known to be induced by H2O2 [22]. H2O2-dependent upregulation of CTT1 expression has been shown to be dependent on the transcription factors Yap1p, Skn7p [23] and Msn2p/Msn4p [24] and it should be pointed out that the minimum H2O2 concentration needed to activate those transcription factors, when using a bolus addition, was found to be 100 μM [25, 26].

Figure 1
figure 1

Low concentrations of H 2 O 2 increase catalase activity in S. cerevisiae. Exponential-phase cells (A) and stationary-phase cells (B) were exposed to the indicated steady-state H2O2 concentrations for 60 min. The values are the mean ± standard deviation of n≥5 independent experiments. The activity of control cells (without added H2O2) was 0.29 ± 0.07 min-1mg-1 for exponential-phase cells and 4.51 ± 0.67 min-1mg-1 for stationary-phase cells. *P < 0.05 vs control; **P < 0.001 vs control.

To define what a high dose of H2O2 is, the survival of S. cerevisiae wild-type cells exposed to steady-state concentrations of H2O2 was determined. For exponential-phase cells, under our conditions, the value of 200 μM can be defined as the border between moderate and high toxic conditions because higher steady-state H2O2 concentrations lead to significant cell death (approximately 55% for 400 μM H2O2 and 80% for 700 μM H2O2) (Figure 2). For stationary-phase cells, doses up to 800 μM may be considered moderate because they did not alter cell survival, which is in agreement with the known higher resistance of these cells to H2O2 when compared to exponential-phase cells [27].

Figure 2
figure 2

Susceptibility of S. cerevisiae cells to steady-state H 2 O 2 -induced oxidative stress. Survival fractions are shown for exponential-phase cells (■) and stationary-phase cells () that were exposed to steady-state H2O2 between 25 μM and 800 μM for 60 min. The values are the mean ± standard deviation of n≥3 independent experiments. *P < 0.05 vs control; **P < 0.01 vs control.

In conclusion, steady-state H2O2 concentrations in the range 20 μM to 50 μM may be viewed as triggering a regulatory H2O2 response in S. cerevisiae.

Low to moderate concentrations of H2O2 do not lead to changes in GAPDH activity in S. cerevisiae exponential-phase cells

GAPDH activity was determined with and without the reducing agent DTT in the assay medium. The difference in the enzyme activity in both assays measures GAPDH reversible inactivation due either to S-glutathionylation, formation of a sulphenic acid or of an intramolecular disulfide. In control cells the activity of GAPDH measured in the absence of DTT was approximately 10% lower than in the presence of DTT (Figure 3A), indicating either that the enzyme was partially oxidized in vivo or that it became oxidized during protein extraction. This partial oxidation of GAPDH in unstressed cells has been previously found [28, 29]. If the reversible inactivation of GAPDH induced by H2O2, namely by S-glutathionylation, has an important role in the regulation of GAPDH activity during oxidative stress it should be expected that a higher reversible inactivation of the enzyme would occur when cells are exposed to low to average H2O2 concentrations (i.e., 20-50 μM, as defined in the previous point).

Figure 3
figure 3

Low H 2 O 2 concentrations do not inactivate GAPDH in S. cerevisiae. GAPDH activity in exponential-phase cells (A, B) or stationary-phase cells (C) treated with either the indicated steady-state H2O2 concentrations for 60 min or (B) with a 2 mM H2O2 bolus addition for 30 min was measured in the presence (closed bars) and in the absence of DTT (dashed bars) in the assay medium. The difference of the activity measured in the presence and in the absence of DTT is a measure of reversible GAPDH thiol oxidation. The values are the mean ± standard deviation of 3≤n < 10 independent experiments. *P < 0.05 vs DTT; #P < 0.01 vs DTT; **P < 0.001 vs control.

When exponential-phase cells were exposed to increasing steady-state H2O2 concentrations no changes in GAPDH activity determined both in the presence and absence DTT were observed for H2O2 concentrations up to 160 μM (Figure 3A). This dose is 8 times higher than the H2O2 concentration identified as being able to induce catalase activity and is close to the steady-state 150 μM H2O2 dose that induces a multi-factorial cellular response causing adaptation to H2O2 [30]. Previous studies of GAPDH inactivation by H2O2 in yeast were done with bolus additions [15, 16, 18, 20], which require the use of a much higher initial H2O2 concentration. When a typical bolus addition of 2 mM H2O2 was added to exponential-phase cells (Figure 3B), after 30 min GAPDH activity had decreased to 10% of that in control cells (1.73 ± 0.10 and 0.17 ± 0.09 U/mg in control and H2O2-treated cells respectively). Part of this inactivation induced by the H2O2 bolus addition was due to reversible GAPDH thiol oxidation since GAPDH activity in H2O2-treated cells measured in the presence of DTT was about 47% of that in control cells (1.99 ± 0.18 and 0.93 ± 0.20 U/mg for control cells and H2O2-treated cells respectively). So, a much higher steady-state concentration of H2O2 (500 μM) was used in order to try to obtain a similar GAPDH inactivation to that observed when using a bolus addition of H2O2. When exponential-phase cells were exposed to a steady-state 500 μM H2O2 concentration, GAPDH activity showed a marked decrease (to 26% and 40% of GAPDH activity in the absence and presence of DTT, respectively) (Figure 3A). However, it should be noted that similarly to what happens with a 2 mM bolus H2O2 addition [16], cell survival when cells are subjected to a steady-state 500 μM H2O2 concentration is lower than 50% (Figure 2).

In conclusion, for cells in the exponential phase GAPDH activity is largely unresponsive to low to moderate H2O2 levels, in opposition to a widely accepted view. GAPDH activity does decrease, but only for H2O2 concentrations that cause significant cell death.

H2O2 does not inactivate irreversibly GAPDH in S. cerevisiae stationary-phase cells

GAPDH activity in stationary-phase cells is about 25% higher than in exponential-phase cells (2.71 ± 0.20 U/mg and 2.03 ± 0.17 U/mg respectively, P < 0.001). No changes in GAPDH activity were found for stationary-phase cells treated with steady-state H2O2 concentrations up to 400 μM (Figure 2C) both in the presence and absence of DTT, when compared with control cells. However, for cells exposed to 400 μM H2O2 there was a significant difference in GAPDH activity determined in the presence and absence of DTT, indicating a small increase in the GAPDH reversible oxidation induced by H2O2. Nevertheless, this H2O2 concentration is much higher than the 50 μM, identified in Figure 1 which induces catalase. Therefore, GAPDH may not be considered to be a sensitive target of H2O2 in stationary phase cells.

Tdh2p/Tdh3p expression is not altered by H2O2 in exponential-phase S. cerevisiae cells

Up until now we have focused on the activity of GAPDH as a whole. Next we evaluate the pattern of expression of each of the three GAPDH isoenzymes. To this end, 2-dimensional gel electrophoresis followed by immune detection was performed (Figures 4, 5 and 6). Previous studies have shown that in two-dimensional gels Tdh2p and Tdh3p slightly overlap, while Tdh1p migrates in a different position [18, 31]. As can be seen in Figure 4 the mouse anti-GAPDH (Chemicon MAB374) reacted only with Tdh2p and Tdh3p (Figure 4A), while the rabbit anti-GAPDH reacted with all three isoforms present in stationary-phase cells (Figure 4C). Tdh1p identification was confirmed using a tdh1 Δ strain (Figure 4D). Tdh1p was not detected in exponential-phase cells (Figure 4B), which is in agreement with previous studies [18, 32, 33] where Tdh1p has been described as a minor GAPDH isoenzyme only expressed in the stationary phase of growth. Tdh1p was also not detected when exponential-phase cells were exposed to 20 μM and 160 μM steady-state H2O2 (results not shown). Since Tdh2p and Tdh3p levels were difficult to obtain from the 2D-analysis, Western blot analysis from SDS-PAGE using the mouse anti-GAPDH followed by signal intensity analysis was used to quantify both Tdh2p and Tdh3p levels when cells were exposed to H2O2. In Figure 5 it can be seen that exposure of exponential-phase cells up to 500 μM H2O2 did not alter the levels of Tdh2p/Tdh3p expression. This contradicts observations obtained with higher H2O2 doses, where a downregulation of Tdh2p/Tdh3p de novo synthesis [34] and Tdh2p/Tdh3p mRNA steady-state levels [35] was observed, and highlights the multitude of possible responses caused by different H2O2 doses.

Figure 4
figure 4

Characterization of the antibodies used for GAPDH detection. Representative (n≥3) two-dimensional analysis of Tdh1p, Tdh2p and Tdh3p (only the region with the 3 GAPDH isoenzymes is shown) S. cerevisiae cells with immunodetection made by Western blot as described in materials and methods are shown. (A) wt stationary-phase cells with identification using mouse anti-GAPDH (Chemicon MAB374). Identification using rabbit anti-GAPDH was performed in (B) wt exponential-phase cells, (C) wt stationary-phase cells, and (D) tdh1 Δ stationary-phase cells.

Figure 5
figure 5

Tdh2p and Tdh3p protein levels are not affected by H 2 O 2 in exponential-phase S. cerevisiae cells. Cells were treated with the steady-state H2O2 concentrations indicated for 60 min. Representative protein loading and immunoblot analysis of Tdh2p/Tdh3p (n = 5) and signal intensity quantification expressed as the mean ± standard deviation in arbitrary units (a.u.) relative to control. Mouse anti-GAPDH that only reacts with Tdh2p and Tdh3p was used for Tdh2p/Tdh3p identification.

Figure 6
figure 6

Low concentrations of H 2 O 2 upregulate Tdh1p and high concentrations downregulate Tdh2p and Tdh3p protein levels in stationary-phase S. cerevisiae cells. Cells were treated with the steady-state H2O2 concentrations indicated for 60 min. (A) Representative protein loading and immunoblot analysis of Tdh2p/Tdh3p (n = 6) and signal intensity quantification expressed as the mean ± standard deviation in arbitrary units (a.u.) relative to control. Mouse anti-GAPDH, which only reacts with Tdh2p and Tdh3p, was used for Tdh2p/Tdh3p identification (see Figure 3). (B) Representative two-dimensional analysis of Tdh1p, Tdh2p and Tdh3p (only the region with the three GAPDH isoenzymes is shown, n≥4) in stationary-phase cells with immunodetection made by Western blot using rabbit anti-GAPDH as described in materials and methods; signal intensity quantification of GAPDH levels normalized to Zwf1p, which was used as internal control, and expressed as the mean ± standard deviation in arbitrary units (a.u.) relative to control is also shown. *P < 0.05 vs control.

H2O2 upregulates Tdh1p expression and downregulates Tdh2p/Tdh3p expression in stationary-phase S. cerevisiae cells

Unlike what happens in exponential-phase cells where exposure to H2O2 does not alter GAPDH expression, in stationary-phase cells a slight downregulation of Tdh2p/Tdh3p expression was observed for higher H2O2 concentrations (Figure 6A). In fact, after exposure to 160 μM H2O2 Tdh2p/Tdh3p steady-state levels were about 80% of those in control cells. On the other hand, Tdh1p expression in stationary-phase cells was upregulated by H2O2 since Tdh1p levels were 3.5 fold higher in cells exposed to steady-state 50 μM H2O2 than in control cells (Figure 6B). Therefore, Tdh1p emerges as a protein that is strongly induced by low concentrations of H2O2 in stationary-phase cells.


It has been established for a number of years that oxidation of particular proteins containing reactive cysteine residues, such as GAPDH, occurs when mammalian and yeast cells are exposed to H2O2. However, in most of these studies, cells are exposed to exogenous H2O2 concentrations several orders of magnitude higher (millimolar) than the physiological concentration [36], due to its rapid removal by intracellular catalases and peroxidases. Therefore, protein oxidation and enzyme inactivation caused by H2O2 has been mostly established for situations when cells were under severe oxidative stress and already dying either by apoptosis or necrosis, and thus very far from a regulatory situation. Much less is known [e.g. [37, 38]] about the effect of H2O2 concentration ranges (micromolar) where H2O2 may affect signaling processes and protein function through reversible changes in protein thiols redox state. In this work, a calibrated method of H2O2 delivery to cells was used where cells were exposed to steady-state concentrations of H2O2 throughout the experiment, which allows the use of much smaller concentrations of H2O2 [21, 39]. This made possible to study for the first time in S. cerevisiae cells how low concentrations of H2O2 affect GAPDH activity and expression. Our study showed that GADPH activity in S. cerevisiae cells, both in the exponential-phase and stationary-phase of growth, is not inhibited by exposure to exogenous low to moderate H2O2 levels. This was unexpected considering previous studies of GAPDH inactivation by H2O2 in yeast [1518, 20] and suggests that in yeast cells exposed to low to moderate H2O2 concentrations the enzymatic systems responsible for the maintenance of cellular protein thiols [20, 40], have enough activity to maintain the SH groups of the reactive cysteine residues in the GAPDH active centre mostly in the reduced form, thus avoiding inactivation of the enzyme. Also, S. cerevisiae exponential-phase cells response to high H2O2 doses includes the upregulation of the proteins involved in the glutaredoxin and thioredoxin systems [34, 41], which are responsible for the reduction of protein disulfides.

Stationary-phase cells have higher resistance to H2O2 than exponential phase cells which is in part due to the higher catalase activity (Figure 2) and also to a lower cellular permeability to H2O2 [27]. So, when exposed to the same exogenous H2O2 concentration stationary-phase cells have a lower intracellular H2O2 concentration than exponential-phase cells [27]. Also, the levels of glutaredoxins [41] and thioredoxins [42] expression are upregulated in the stationary phase of growth. This probably partially explains why in stationary-phase cells overall GAPDH activity is not inhibited for the whole range of H2O2 concentrations used in this work. Unlike what happens for exponential-phase cells, where Tdh2p and Tdh3p levels are not altered by exposure to H2O2 and Tdh1p is not detected, in stationary-phase cells Tdh2p and Tdh3p levels were slightly downregulated at higher H2O2 concentrations. In spite of this result, overall GAPDH activity and total GAPDH mRNA steady-state levels in stationary-phase cells are not altered by H2O2 (results not shown). A possible explanation for this discrepancy is that, in spite of the decrease in the total amount of Tdh3p plus Tdh2p, the relative proportion of Tdh2p versus Tdh3p is increased. It is known that the three isoenzymes have different kinetic constants since it has been determined that Tdh3p has a two- to three-fold lower apparent Vmax than Tdh2p [11]. Also, it can be hypothesized that Tdh1p upregulation observed at low H2O2 concentrations is compensating for the decreased levels of Tdh2p/Tdh3p, the overall net result being that GAPDH activity is maintained constant.

Tdh1p levels have also been previously found to be induced by reductive stress caused by an excess of cytoplasmic NADH in an anaerobically grown gpd2 Δ strain lacking one of the glycerol-3-phosphate dehydrogenases [43]. This upregulation of Tdh1p expression by changes in cellular redox state may be related to its function in signaling pathways, possibly the Hog1p pathway. In fact, in Schizosaccharomyces pombe, a recent study [44] showed that in response to H2O2 stress, the Cys-152 of Tdh1p is transiently oxidized. This oxidation enhances the association of Tdh1p with Mcs4p (mitotic catastrophe suppressor) and Mpr1p, a protein that transfers a phosphoryl group from the Mak2/Mak3 sensor histidine kinases activated by H2O2. The equivalent pathway in S. cerevisiae is the Hog1p pathway involved in the response to increased extracellular osmolarity, which is also activated by oxidative stress [45, 46].

In the last years the paradigm found in the literature is that GAPDH is a sensitive protein target of H2O2 and that its inhibition by H2O2 is a controlled response advantageous for cells because it diverts glucose from the glycolytic pathway to the pentose phosphate pathway, thus increasing the availability of NADPH for antioxidant enzymes [12, 15, 47]. In favor of such an hypothesis, a recent study [48] found that H2O2-induced GAPDH inactivation to about 20% of control resulted in an increase in the levels of the metabolites of the pentose phosphate pathway. Also, a mathematical model indicated that for those levels of GAPDH inhibition there was a change in the NADPH/NADP+ ratio from 6.5 to 19, with a steep increase in the ratio for levels of GAPDH inactivation greater than about 40%. Ralser et al. [48] used that evidence as support of a model where GAPDH functions as a cellular switch that reroutes the carbohydrate flux to maintain the cytoplasmic NADPH/NADP+ equilibrium to counteract oxidative stress. However, as shown by this work, those levels of GAPDH inactivation can only be attained under severe oxidative stress when cells are dying. Therefore, this rerouting of the glycolytic carbohydrate flux due to GAPDH inhibition, although it may be important in pathophysiological situations, is not a physiological regulatory response. Moreover, the higher GAPDH activity observed after exhaustion of carbon sources in stationary-phase cells when compared to glucose-based growth in exponential-phase cells argues against the rerouting of carbohydrate flux being an important physiological mechanism. This higher GAPDH activity in stationary-phase cells also supports the paradigm [8, 9] that GAPDH has other functions in the cell besides its role in glycolysis.


In conclusion, this work has shown that in S. cerevisiae GAPDH activity is largely unresponsive to low to moderate doses of H2O2. This highlights the importance of studies of H2O2-induced oxidative stress using concentrations closer to the physiological for determining the importance of protein oxidation phenomena in the regulation of cellular metabolism. Most other studies of GAPDH in yeast have used considerably higher concentrations of H2O2 than we used which lead to conclusions that are possibly only important in situations of necrosis and apoptosis. The notable exception to the lack of GAPDH response to low H2O2 concentrations is the H2O2-induced upregulation of Tdh1p expression in stationary-phase S. cerevisiae cells.


Compounds, antibodies and other materials

Yeast extract, bactopeptone, yea < st nitrogen base and agar were from Difco, Detroit, MI, USA. Glucose oxidase (Aspergillus niger) and digitonin were from Aldrich, Steinheim, Germany. D, L-glyceraldehyde-3-phoshate, L-α-amino acid oxidase (Crotalus atrox), bovine liver catalase and phenylmethylsulfonyl fluoride were from Sigma Chemical Company, St. Louis, MO, USA. Hydrogen peroxide was obtained from Merck & Co., Inc., Whitehouse Station, NJ, USA. Anti-glyceraldehyde-3-phoshate dehydrogenase monoclonal antibody was from Chemicon International Inc., Temecula, CA, USA and rabbit anti-glyceraldehyde-3-phoshate dehydrogenase antibody was a kind gift from Dr. Pedro Moradas-Ferreira, Instituto de Biologia Molecular e Celular, Porto, Portugal. Anti-mouse IgG-horseradish peroxidase conjugate antibody (sc-2005) and anti-rabbit IgG-horseradish peroxidase conjugate antibody (sc-2004) were obtained from Santa Cruz Biotechnology, Inc., Santa Cruz, CA, USA).

Yeast strains, media and growth conditions

The S. cerevisiae strains used in this work, BY4741 (MATa; his3Δ1; leu2Δ0; met15Δ0; ura3Δ0) and tdh1 Δ (isogenic to BY4741 with YJL052w::kanMX4), were obtained from EUROSCARF, Frankfurt, Germany. For all experiments S. cerevisiae cells were inoculated at an OD600 of 0.05 and cultured in synthetic complete (SC) medium containing 6.8% (w/v) yeast nitrogen base, 2% (w/v) glucose, and amino acids as indicated in [49], at 30°C and with shaking at 160 rpm. Exponential-phase cells were harvested at 0.5 OD600 (~2 × 107 cells) and stationary-phase cells were harvested after 7 days.

Exposure to H2O2 and cell survival

Exponential-phase cells were exposed to steady-state H2O2 concentrations during 60 min in fresh SC medium at 30°C with shaking at 160 rpm using glucose oxidase [30]. For stationary-phase cells, cells were resuspended in an amino acid solution (0.1 M phosphate buffer, pH 7.4, containing amino acids with the same concentrations as in SC medium) and L-α-amino acid oxidase was used for H2O2 generation [27]. Briefly, an aliquot containing the desired H2O2 concentration was added to the cells together with either glucose oxidase or L-α-amino acid oxidase at such an activity that the rapid consumption of the added initial H2O2 concentration by the cells was compensated, thus keeping H2O2 concentration constant (steady-state) during the assay. Cell survival after exposure to steady-state concentrations of H2O2 was monitored by plating diluted sample aliquots on YPD plates [50] and counting colonies after 48 h.

Protein extracts

Crude protein extracts were prepared by glass bead lysis. Cells were suspended either in 100 mM potassium phosphate buffer pH 7.4 containing 1 mM PMSF or, in the case of two-dimensional gel electrophoresis analysis, in Tris HCl 10 mM buffer pH 8.0 containing 2 μM DTT, protease inhibitors: 1 mM PMSF, 1.5 μg/ml benzamidine, 10 μg/ml leupeptin, and 1 μg/ml pepstatin, added to an equal volume of glass beads, and vortexed for 7 cycles of 1 min of vortexing followed by 1 min of cooling on ice. The mixture was then centrifuged at 8000 × g, 20 min at 8°C. The supernatants were used for determinations of enzyme activities, total protein [51] and GAPDH levels by Western blot after SDS-PAGE or two-dimensional gel electrophoresis.

Enzyme activities

Glyceraldehyde-3-phosphate dehydrogenase activity in protein extracts was assayed according to [52], with some minor modifications. NADH formation was measured at 340 nm (ε = 6220 M-1cm-1) during 4 min at 25°C in 1 ml reaction medium with 0.015 M sodium pyrophosphate buffer pH 8.5 containing 0.03 M sodium arsenate, 0.26 mM NAD+, 3.5 mM dithiothreitol (DTT) and protein extract. The reaction was started by the addition of 0.525 mM DL-glyceraldehyde-3-phosphate. The activity assay was also performed in the absence of DTT. One unit is defined as the quantity of enzyme reducing 1 μmol NAD+/min at 25°C and pH 8.5.

In exponential-phase cells catalase activity was determined in situ. Cell membrane permeabilization was achieved by incubating cells with 0.02% (w/v) digitonin, dissolved in dimethylsulphoxide, in 0.1 M potassium phosphate buffer, pH 6.5, for 15 min at 30°C with shaking. H2O2 consumption (100 μM initial concentration) by permeabilized cells suspended in the permeabilization buffer at 30°C was followed using an oxygen electrode (Hansatech Instruments Ltd, Norfolk, England). In stationary-phase cells catalase activity was measured spectrophotometrically in protein extracts by following H2O2 consumption (initial concentration, 10 mM) at 240 nm at 25°C for 2 min according to Aebi [53]. H2O2 concentrations were plotted on a semi-logarithmic graph against time and the first order rate constant (catalase activity) was calculated.

SDS-PAGE and two-dimensional gel electrophoresis

SDS-PAGE was carried out according to [54]. 50 μg of total proteins were denaturated and analyzed in 7.5% (w/v) polyacrylamide (w/v). For two-dimensional analysis overnight precipitation using acetone (1 ml) was done to protein extracts (150 μg total protein). The pellet was resuspended in 250 μl of rehydration solution [8 M urea, 0.5% (w/v) CHAPS, 0.2% (w/v) DTT, 0.5% (v/v) IPG buffer pH 3-10, 0.002% (w/v) bromophenol blue], were loaded into the strip holders (Amersham Biosciences) and IEF (first dimension) was carried out on linear IPGs (pH 3-10; 13 cm long IPG) and achieved using the Ettan IPGphor system (GE Healthcare). Strips were rehydrated with 150 μg of proteins extracts for 12 h at room temperature. Strips were then focused according to the following electrical conditions at 20°C: 150 V for 1 h, 300 V for 1 h, 600 V for 1 h, from 600 to 4000 V in 90 min and 4000 V for 4 h. After focusing IPG strips were placed for 15 min in equilibration buffer [6 M urea, 30% (v/v) glycerol, 2% (w/v) SDS, 0.05 M Tris-HCl, pH 8.8, 0.002% (w/v) bromophenol blue] containing 1% (w/v) DTT and, subsequently, for 15 min in the same buffer but replacing the 1% (w/v) DTT by 2.5% (w/v) iodoacetamide [54]. The second dimension was carried out on 10% polyacrylamide gradient gels (16 × 14 × 0.15 cm) at 55 V per gel and 21°C until the dye front reached the bottom of the gel, according to Laemmli [54]. Identification of Tdh1p, Tdh2p and Tdh3p in protein extracts from wt and tdh1 Δ cells after SDS-PAGE or two-dimensional gel electrophoresis was made by Western blot as described below.

Western blot analysis

For immunodetection, the proteins were transferred to nitrocellulose membrane (0.45 nm; Schleicher and Schuell) in a semi-dry system, using 39 mM glycine, 48 mM Tris, 0.0375% (w/v) SDS and 20% (v/v) methanol pH 9.2 as transfer buffer [55], during 60 min at 0.8 mA/cm2, not exceeding 25 V. Blots were blocked at room temperature for 1 h in PBS (4.3 mM Na2HPO4, 1.4 mM KH2PO4, 137 mM NaCl and 2.0 mM KCl, pH 7.4) containing 5% (w/v) fat-free milk powder, before incubation with the primary antibody. The mouse anti-GAPDH (Chemicon MAB374) was used with a dilution of 1:1000 whereas the rabbit anti-GAPDH was used with a dilution of 1:5000, followed by incubation for 1 h. After washing 5 times in PBS containing 0.1% (v/v) Tween-20, the blots were incubated for 1 h with the secondary antibody conjugated to horseradish peroxidase (sc-2005; 1:2000 or sc-2004; 1:5000), washed extensively with PBS and detected by enhanced chemiluminescence (ECL kit, Amersham). Protein levels were quantified by signal intensity analysis by using ImageJ [56], normalized to the protein loading, either membrane stained with Ponceau S when doing SDS-PAGE, or Zwf1p levels, and expressed as arbitrary units relative to control. For stationary-phase cells Zwf1p was used as internal control since its expression is not altered by the H2O2 concentrations used in this study (Cyrne et al., unpublished).

Statistical analysis

Results presented are the means ± standard deviation of the indicated independent experiments. To determine statistical significance among groups data were analyzed using one-way analysis of variance (ANOVA) followed by post analysis with the Tukey-Kramer multiple comparisons test or, alternatively, when appropriate, Student's t-test.





Glyceraldehyde-3-phosphate dehydrogenase

S. Cerevisiae :

Saccharomyces cerevisiae

SC medium:

synthetic complete medium


  1. Winterbourn CC, Hampton MB: Thiol chemistry and specificity in redox signaling. Free Radic Biol Med. 2008, 45: 549-561. 10.1016/j.freeradbiomed.2008.05.004.

    Article  PubMed  Google Scholar 

  2. Janssen-Heininger YM, Mossman BT, Heintz NH, Forman HJ, Kalyanaraman B, Finkel T, Stamler JS, Rhee SG, van der Vliet A: Redox-based regulation of signal transduction: principles, pitfalls, and promises. Free Radic Biol Med. 2008, 45: 1-17. 10.1016/j.freeradbiomed.2008.03.011.

    Article  PubMed  PubMed Central  Google Scholar 

  3. Claiborne A, Yeh JI, Mallett TC, Luba J, Crane EJ, Charrier V, Parsonage D: Protein-sulfenic acids: diverse roles for an unlikely player in enzyme catalysis and redox regulation. Biochemistry. 1999, 38: 15407-15416. 10.1021/bi992025k.

    Article  PubMed  Google Scholar 

  4. Saurin AT, Neubert H, Brennan JP, Eaton P: Widespread sulfenic acid formation in tissues in response to hydrogen peroxide. Proc Natl Acad Sci USA. 2004, 101: 17982-17987. 10.1073/pnas.0404762101.

    Article  PubMed  PubMed Central  Google Scholar 

  5. Rhee SG, Jeong W, Chang TS, Woo HA: Sulfiredoxin, the cysteine sulfinic acid reductase specific to 2-Cys peroxiredoxin: its discovery, mechanism of action, and biological significance. Kidney Int Suppl. 2007, S3-S8. 10.1038/

    Google Scholar 

  6. Cumming RC, Schubert D: Amyloid-beta induces disulfide bonding and aggregation of GAPDH in Alzheimer's disease. FASEB J. 2005, 19: 2060-2062.

    PubMed  Google Scholar 

  7. Haynes CM, Titus EA, Cooper AA: Degradation of misfolded proteins prevents ER-derived oxidative stress and cell death. Mol Cell. 2004, 15: 767-776. 10.1016/j.molcel.2004.08.025.

    Article  PubMed  Google Scholar 

  8. Sirover MA: New nuclear functions of the glycolytic protein, glyceraldehyde-3-phosphate dehydrogenase, in mammalian cells. J Cell Biochem. 2005, 95: 45-52. 10.1002/jcb.20399.

    Article  PubMed  Google Scholar 

  9. Nakajima H, Amano W, Kubo T, Fukuhara A, Ihara H, Azuma YT, Tajima H, Inui T, Sawa A, Takeuchi T: Glyceraldehyde-3-phosphate dehydrogenase aggregate formation participates in oxidative stress-induced cell death. J Biol Chem. 2009, 284: 34331-34341. 10.1074/jbc.M109.027698.

    Article  PubMed  PubMed Central  Google Scholar 

  10. McAlister L, Holland MJ: Isolation and characterization of yeast strains carrying mutations in the glyceraldehyde-3-phosphate dehydrogenase genes. J Biol Chem. 1985, 260: 15013-15018.

    PubMed  Google Scholar 

  11. McAlister L, Holland MJ: Differential expression of the three yeast glyceraldehyde-3-phosphate dehydrogenase genes. J Biol Chem. 1985, 260: 15019-15027.

    PubMed  Google Scholar 

  12. Ravichandran V, Seres T, Moriguchi T, Thomas JA, Johnston RB: S-thiolation of glyceraldehyde-3-phosphate dehydrogenase induced by the phagocytosis-associated respiratory burst in blood monocytes. J Biol Chem. 1994, 269: 25010-25015.

    PubMed  Google Scholar 

  13. Schuppe-Koistinen I, Moldeus P, Bergman T, Cotgreave IA: S-thiolation of human endothelial cell glyceraldehyde-3-phosphate dehydrogenase after hydrogen peroxide treatment. Eur J Biochem. 1994, 221: 1033-1037. 10.1111/j.1432-1033.1994.tb18821.x.

    Article  PubMed  Google Scholar 

  14. Hwang NR, Yim SH, Kim YM, Jeong J, Song EJ, Lee Y, Lee JH, Choi S, Lee KJ: Oxidative modifications of glyceraldehyde-3-phosphate dehydrogenase play a key role in its multiple cellular functions. Biochem J. 2009, 423: 253-264. 10.1042/BJ20090854.

    Article  PubMed  Google Scholar 

  15. Grant CM, Quinn KA, Dawes IW: Differential protein S-thiolation of glyceraldehyde-3-phosphate dehydrogenase isoenzymes influences sensitivity to oxidative stress. Mol Cell Biol. 1999, 19: 2650-2656.

    Article  PubMed  PubMed Central  Google Scholar 

  16. Shenton D, Grant CM: Protein S-thiolation targets glycolysis and protein synthesis in response to oxidative stress in the yeast Saccharomyces cerevisiae. Biochem J. 2003, 374: 513-519. 10.1042/BJ20030414.

    Article  PubMed  PubMed Central  Google Scholar 

  17. Cabiscol E, Piulats E, Echave P, Herrero E, Ros J: Oxidative stress promotes specific protein damage in Saccharomyces cerevisiae. J Biol Chem. 2000, 275: 27393-27398.

    PubMed  Google Scholar 

  18. Costa VM, Amorim MA, Quintanilha A, Moradas-Ferreira P: Hydrogen peroxide-induced carbonylation of key metabolic enzymes in Saccharomyces cerevisiae: the involvement of the oxidative stress response regulators Yap1 and Skn7. Free Radic Biol Med. 2002, 33: 1507-1515. 10.1016/S0891-5849(02)01086-9.

    Article  PubMed  Google Scholar 

  19. Yoo BS, Regnier FE: Proteomic analysis of carbonylated proteins in two-dimensional gel electrophoresis using avidin-fluorescein affinity staining. Electrophoresis. 2004, 25: 1334-1341. 10.1002/elps.200405890.

    Article  PubMed  Google Scholar 

  20. Shenton D, Perrone G, Quinn KA, Dawes IW, Grant CM: Regulation of protein S-thiolation by glutaredoxin 5 in the yeast Saccharomyces cerevisiae. J Biol Chem. 2002, 277: 16853-16859. 10.1074/jbc.M200559200.

    Article  PubMed  Google Scholar 

  21. Oliveira-Marques V, Marinho HS, Cyrne L, Antunes F: Role of hydrogen peroxide in NF-kappaB activation: from inducer to modulator. Antioxid Redox Signal. 2009, 11: 2223-2243. 10.1089/ars.2009.2601.

    Article  PubMed  Google Scholar 

  22. Izawa S, Inoue Y, Kimura A: Importance of catalase in the adaptive response to hydrogen peroxide: analysis of acatalasaemic Saccharomyces cerevisiae. Biochem J. 1996, 320: 61-67.

    Article  PubMed  PubMed Central  Google Scholar 

  23. Lee J, Godon C, Lagniel G, Spector D, Garin J, Labarre J, Toledano MB: Yap1 and Skn7 control two specialized oxidative stress response regulons in yeast. J Biol Chem. 1999, 274: 16040-16046. 10.1074/jbc.274.23.16040.

    Article  PubMed  Google Scholar 

  24. Martinez-Pastor MT, Marchler G, Schuller C, Marchler-Bauer A, Ruis H, Estruch F: The Saccharomyces cerevisiae zinc finger proteins Msn2p and Msn4p are required for transcriptional induction through the stress response element (STRE). EMBO J. 1996, 15: 2227-2235.

    PubMed  PubMed Central  Google Scholar 

  25. Delaunay A, Isnard AD, Toledano MB: H2O2 sensing through oxidation of the Yap1 transcription factor. EMBO J. 2000, 19: 5157-5166. 10.1093/emboj/19.19.5157.

    Article  PubMed  PubMed Central  Google Scholar 

  26. Boisnard S, Lagniel G, Garmendia-Torres C, Molin M, Boy-Marcotte E, Jacquet M, Toledano MB, Labarre J, Chedin S: H2O2 activates the nuclear localization of Msn2 and Maf1 through thioredoxins in Saccharomyces cerevisiae. Eukaryot Cell. 2009, 8: 1429-1438. 10.1128/EC.00106-09.

    Article  PubMed  PubMed Central  Google Scholar 

  27. Sousa-Lopes A, Antunes F, Cyrne L, Marinho HS: Decreased cellular permeability to H2O2 protects Saccharomyces cerevisiae cells in stationary phase against oxidative stress. FEBS Lett. 2004, 578: 152-156. 10.1016/j.febslet.2004.10.090.

    Article  PubMed  Google Scholar 

  28. Le Moan N, Clement G, Le Maout S, Tacnet F, Toledano MB: The Saccharomyces cerevisiae proteome of oxidized protein thiols: contrasted functions for the thioredoxin and glutathione pathways. J Biol Chem. 2006, 281: 10420-10430. 10.1074/jbc.M513346200.

    Article  PubMed  Google Scholar 

  29. McDonagh B, Ogueta S, Lasarte G, Padilla CA, Barcena JA: Shotgun redox proteomics identifies specifically modified cysteines in key metabolic enzymes under oxidative stress in Saccharomyces cerevisiae. J Proteomics. 2009, 72: 677-689. 10.1016/j.jprot.2009.01.023.

    Article  PubMed  Google Scholar 

  30. Branco MR, Marinho HS, Cyrne L, Antunes F: Decrease of H2O2 plasma membrane permeability during adaptation to H2O2 in Saccharomyces cerevisiae. J Biol Chem. 2004, 279: 6501-6506. 10.1074/jbc.M311818200.

    Article  PubMed  Google Scholar 

  31. Norbeck J, Blomberg A: Two-dimensional electrophoretic separation of yeast proteins using a non-linear wide range (pH 3-10) immobilized pH gradient in the first dimension; reproducibility and evidence for isoelectric focusing of alkaline (pI > 7) proteins. Yeast. 1997, 13: 1519-1534. 10.1002/(SICI)1097-0061(199712)13:16<1519::AID-YEA211>3.0.CO;2-U.

    Article  PubMed  Google Scholar 

  32. Boucherie H, Bataille N, Fitch IT, Perrot M, Tuite MF: Differential synthesis of glyceraldehyde-3-phosphate dehydrogenase polypeptides in stressed yeast cells. FEMS Microbiol Lett. 1995, 125: 127-133. 10.1111/j.1574-6968.1995.tb07348.x.

    Article  PubMed  Google Scholar 

  33. Delgado ML, O'Connor JE, Azorin I, Renau-Piqueras J, Gil ML, Gozalbo D: The glyceraldehyde-3-phosphate dehydrogenase polypeptides encoded by the Saccharomyces cerevisiae TDH1, TDH2 and TDH3 genes are also cell wall proteins. Microbiology. 2001, 147: 411-417.

    Article  PubMed  Google Scholar 

  34. Godon C, Lagniel G, Lee J, Buhler J-M, Kieffer S, Perrot M, Boucherie H, Toledano MB, Labarre J: The H2O2 stimulon in Saccharomyces cerevisiae. J Biol Chem. 1998, 273: 22480-22489. 10.1074/jbc.273.35.22480.

    Article  PubMed  Google Scholar 

  35. Gasch AP, Spellman PT, Kao CM, Carmel-Harel O, Eisen MB, Storz G, Botstein D, Brown PO: Genomic expression programs in the response of yeast cells to environmental changes. Mol Biol Cell. 2000, 11: 4241-4257.

    Article  PubMed  PubMed Central  Google Scholar 

  36. Halliwell B, Clement MV, Long LH: Hydrogen peroxide in the human body. FEBS Lett. 2000, 486: 10-13. 10.1016/S0014-5793(00)02197-9.

    Article  PubMed  Google Scholar 

  37. Baty JW, Hampton MB, Winterbourn CC: Proteomic detection of hydrogen peroxide-sensitive thiol proteins in Jurkat cells. Biochem J. 2005, 389: 785-795. 10.1042/BJ20050337.

    Article  PubMed  PubMed Central  Google Scholar 

  38. Cumming RC, Andon NL, Haynes PA, Park M, Fischer WH, Schubert D: Protein disulfide bond formation in the cytoplasm during oxidative stress. J Biol Chem. 2004, 279: 21749-21758. 10.1074/jbc.M312267200.

    Article  PubMed  Google Scholar 

  39. Antunes F, Cadenas E: Cellular titration of apoptosis with steady-state concentrations of H2O2. Sub-micromolar levels of H2O2 induce apoptosis through Fenton chemistry independent of cellular thiol state. Free Radic Biol Med. 2001, 30: 1008-1018. 10.1016/S0891-5849(01)00493-2.

    Article  PubMed  Google Scholar 

  40. Greetham D, Vickerstaff J, Shenton D, Perrone GG, Dawes IW, Grant CM: Thioredoxins function as deglutathionylase enzymes in the yeast Saccharomyces cerevisiae. BMC Biochem. 2010, 11: 3-10.1186/1471-2091-11-3.

    Article  PubMed  PubMed Central  Google Scholar 

  41. Luikenhuis S, Perrone G, Dawes IW, Grant CM: The yeast Saccharomyces cerevisiae contains two glutaredoxin genes that are required for protection against reactive oxygen species. Mol Biol Cell. 1998, 9: 1081-1091.

    Article  PubMed  PubMed Central  Google Scholar 

  42. Garrido EO, Grant CM: Role of thioredoxins in the response of Saccharomyces cerevisiae to oxidative stress induced by hydroperoxides. Mol Microbiol. 2002, 43: 993-1003. 10.1046/j.1365-2958.2002.02795.x.

    Article  PubMed  Google Scholar 

  43. Valadi H, Valadi A, Ansell R, Gustafsson L, Adler L, Norbeck J, Blomberg A: NADH-reductive stress in Saccharomyces cerevisiae induces the expression of the minor isoform of glyceraldehyde-3-phosphate dehydrogenase (TDH1). Curr Genet. 2004, 45: 90-95. 10.1007/s00294-003-0469-1.

    Article  PubMed  Google Scholar 

  44. Morigasaki S, Shimada K, Ikner A, Yanagida M, Shiozaki K: Glycolytic enzyme GAPDH promotes peroxide stress signaling through multistep phosphorelay to a MAPK cascade. Mol Cell. 2008, 30: 108-113. 10.1016/j.molcel.2008.01.017.

    Article  PubMed  PubMed Central  Google Scholar 

  45. Singh KK: The Saccharomyces cerevisiae Sln1p-Ssk1p two-component system mediates response to oxidative stress and in an oxidant-specific fashion. Free Radic Biol Med. 2000, 29: 1043-1050. 10.1016/S0891-5849(00)00432-9.

    Article  PubMed  Google Scholar 

  46. Bilsland E, Molin C, Swaminathan S, Ramne A, Sunnerhagen P: Rck1 and Rck2 MAPKAP kinases and the HOG pathway are required for oxidative stress resistance. Mol Microbiol. 2004, 53: 1743-1756. 10.1111/j.1365-2958.2004.04238.x.

    Article  PubMed  Google Scholar 

  47. Grant CM: Metabolic reconfiguration is a regulated response to oxidative stress. J Biol. 2008, 7: 1-10.1186/jbiol63.

    Article  PubMed  PubMed Central  Google Scholar 

  48. Ralser M, Wamelink MM, Kowald A, Gerisch B, Heeren G, Struys EA, Klipp E, Jakobs C, Breitenbach M, Lehrach H: Dynamic rerouting of the carbohydrate flux is key to counteracting oxidative stress. J Biol. 2007, 6: 10-10.1186/jbiol61.

    Article  PubMed  PubMed Central  Google Scholar 

  49. Folmer V, Pedroso N, Matias AC, Lopes SCDN, Antunes F, Cyrne L, Marinho HS: H2O2 induces rapid biophysical and permeability changes in the plasma membrane of Saccharomyces cerevisiae. Biochim Biophys Acta. 2008, 1778: 1141-1147. 10.1016/j.bbamem.2007.12.008.

    Article  PubMed  Google Scholar 

  50. Johnston JR: Molecular Genetics of Yeast. A practical approach. Edited by: Johnston JR. 1994, New York: IRL Press, 261-265.

    Google Scholar 

  51. Peterson GL: A simplification of the protein assay method of Lowry et al. which is more generally applicable. Anal Biochem. 1977, 83: 346-356. 10.1016/0003-2697(77)90043-4.

    Article  PubMed  Google Scholar 

  52. Velick SF: Glyceraldehyde-3-Phosphate Dehydrogenase from Muscle. Methods Enzymol. 1955, 1: 401-406. full_text.

    Article  Google Scholar 

  53. Aebi HE: Catalase. Methods of Enzymatic Analysis. Edited by: Bergmeyer HU. 1984, Weinheim: Verlag Chemie, 273-284.

    Google Scholar 

  54. Laemmli UK: Cleavage of structural proteins during the assembly of the head of bacteriophage T4. Nature. 1970, 227: 680-685. 10.1038/227680a0.

    Article  PubMed  Google Scholar 

  55. Bjerrum OJ, Schafer-Nielsen C: Analytical Electrophoresis. Edited by: Dunn MJ. 1986, Weinheim: Verlag Chemie, 315-

    Google Scholar 

  56. Rasband WS: ImageJ. 1997, U. S. National Institutes of Health, Bethesda, Maryland, USA

    Google Scholar 

Download references


This work was supported by Fundação para a Ciência e a Tecnologia (FCT), Portugal pluriannual funding. We would like to thank Prof. Pedro Moradas-Ferreira (Instituto de Biologia Molecular e Celular, Porto, Portugal) for the kind gift of the rabbit anti-GAPDH antibody, and Dr. Armindo Salvador (Centro de Neurociências e Biologia Celular, Universidade de Coimbra, Portugal) for helpful discussions.

Author information

Authors and Affiliations


Corresponding author

Correspondence to H Susana Marinho.

Additional information

Authors' contributions

LC, FA and HSM conceived the study, and participated in its design and coordination. LC performed the 2D-electrophoresis and western blot analysis. FA performed the steady-state H2O2 exposure of cells and helped to draft the manuscript. ASL, JDB and HSM performed the enzyme activity assays. HSM analyzed and interpreted the data and drafted the manuscript. All authors read and approved the final manuscript.

Authors’ original submitted files for images

Rights and permissions

Open Access This article is published under license to BioMed Central Ltd. This is an Open Access article is distributed under the terms of the Creative Commons Attribution License ( ), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Reprints and permissions

About this article

Cite this article

Cyrne, L., Antunes, F., Sousa-Lopes, A. et al. Glyceraldehyde-3-phosphate dehydrogenase is largely unresponsive to low regulatory levels of hydrogen peroxide in Saccharomyces cerevisiae. BMC Biochem 11, 49 (2010).

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: