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BIOCHEMICAL PROCESSES AND MACROMOLECULAR STRUCTURES

Naphthoquinone-Dependent Generation of Superoxide Radicals by Quinone Reductase Isolated from the Plasma Membrane of Soybean^[W]

Universität Freiburg, Institut für Biologie II, D–79104 Freiburg, Germany (P.S., F.D.); and Commissariat à l'Energie Atomique, Institut de Biologie et Technologies de Saclay, CNRS Unité de Recherche Associée 2096, Service de Bioénergétique Biologie Structurale et Mécanisme, F–91191 Gif-sur-Yvette cedex, France (E.H., A.K.-L.)

	ABSTRACT

TOP ABSTRACT RESULTS AND DISCUSSION MATERIALS AND METHODS LITERATURE CITED

 
Using a tetrazolium-based assay, a NAD(P)H oxidoreductase was purified from plasma membranes prepared from soybean (Glycine max) hypocotyls. The enzyme, a tetramer of 85 kD, produces O₂^·– by a reaction that depended on menadione or several other 1,4-naphthoquinones, in apparent agreement with a classification as a one-electron-transferring flavoenzyme producing semiquinone radicals. However, the enzyme displayed catalytic and molecular properties of obligatory two-electron-transferring quinone reductases of the DT-diaphorase type, including insensitivity to inhibition by diphenyleneiodonium. This apparent discrepancy was clarified by investigating the pH-dependent reactivity of menadionehydroquinone toward O₂ and identifying the protein by mass spectrometry and immunological techniques. The enzyme turned out to be a classical NAD(P)H:quinone-acceptor oxidoreductase (EC 1.6.5.2, formerly 1.6.99.2) that reduces menadione to menadionehydroquinone and subsequently undergoes autoxidation at pH 6.5. Autoxidation involves the production of the semiquinone as an intermediate, creating the conditions for one-electron reduction of O₂. The possible function of this enzyme in the generation of O₂^·– and H₂O₂ at the plasma membrane of plants in vivo is discussed.

In this context, it is of particular interest to know whether the plasma membrane redox system is capable of transferring electrons from NAD(P)H to O₂ and whether such an activity is involved in the generation of reactive oxygen species at the outer membrane face (Murphy and Auh, 1996; van Gestelen et al., 1997; Vuleti et al., 2003). Based on molecular genetic studies, this capacity is generally attributed to the "respiratory burst oxidase" homologues (RBOHs; i.e. plant equivalents to the NADPH oxidase [NOX] of mammalian phagocytes) that catalyze a transmembrane electron transport from NADPH to O₂ via FAD and cytochrome (Cyt) b₅₅₈, resulting in the formation of superoxide radicals (O₂^·–; Sumimoto et al., 2005). So far, the expression of RBOH genes in plants has been studied mainly at the level of transcription. Moreover, Arabidopsis (Arabidopsis thaliana) mutants defective in one or another member of the RBOH family have been characterized (Torres and Dangl, 2005; Gapper and Dolan, 2006). Using antibodies raised against RBOH peptides, RBOH proteins have been identified by immunoblotting in plasma membranes from several plant species (Keller et al., 1998; Sagi and Fluhr, 2001; Simon-Plas et al., 2002) and by in situ imaging of GFP-RBOH fusion protein (Kobayashi et al., 2006). However, RBOH proteins have not yet been isolated from plants, and their catalytic properties and cofactor requirements are still largely unknown. The ability of diphenylene iodonium (DPI) to inhibit mammalian NOX at low concentrations (<10 µM; Doussiere and Vignais, 1992) has often been used as a diagnostic feature for NOX activity in plant cells or cell fractions, although DPI also inhibits other flavin- or heme-containing enzymes, especially at higher concentrations (10 µM; Frahry and Schopfer, 1998; Doussiere et al., 1999); therefore, it is no suitable tool to unequivocally identify NOX enzymes.

Attempts to isolate proteins with O₂^·– synthase activity from plasma membranes by biochemical methods have not yet led to homogeneous results. van Gestelen et al. (1997) separated an O₂^·–-producing, FMN-containing protein fraction from FeCN/DCPIP oxidoreductases in solubilized Phaseolus plasma membranes. No cytochrome was detected. O₂^·– generation was much higher with NADPH than with NADH and could be inhibited by DPI, although only at high concentrations (60 µM for 50% inhibition). The O₂^·–-producing activity of plasma membrane vesicles was strongly elevated by 1,4-naphthoquinones (NQs) such as juglone, and the active proteins could be divided by ion exchange chromatography into a NADPH-specific, NQ-independent fraction and three NQ-dependent fractions (van Gestelen et al., 1998). The main NQ-dependent fraction showed high specificity for NADH compared with NADPH. The plasma membrane reduced Cyt c at pH 6 in a juglone-stimulated manner, leading to the conclusion that semiquinones are involved in the catalytic cycle.

Using Rosa cells as a source of plasma membranes, Murphy et al. (2000) partly purified an O₂^·–-producing enzyme activity that showed apparent specificity for either NADH or NADPH, depending on whether lucigenin luminescence or Cyt c reduction was used to assay O₂^·– formation. Spectroscopic evidence indicated the presence of pterin rather than flavin in the preparation. The activity was stimulated by NQ (menadione [MD]) and strongly inhibited by DPI (0.5 µM for 50% inhibition) and NaN₃ but not by KCN.

Taken together, this fragmentary experimental evidence illustrates that the enzymatic mechanism(s) for O₂^·– generation in the plant plasma membrane may be more complex than suggested by the concept modeled on phagocyte NOX. In an attempt to elucidate this complex picture, we are investigating the molecular and catalytic properties of NAD(P)H-oxidizing enzymes that are potentially involved in O₂^·– generation by plasma membranes isolated from soybean (Glycine max) hypocotyls. In this article, we describe an enzyme that is responsible for the NQ-stimulated production of O₂^·– in these membranes. O₂^·–-producing activity was measured using the tetrazolium compound Na,3'-(1-[phenylamino-carbonyl]-3,4-tetrazolium)-bis(4-methoxy-6-nitro)benzenesulfonic acid hydrate (XTT), which can be reduced by O₂^·– to a photometrically detectable formazan (Able et al., 1998). To analyze the reaction mechanism of O₂^·– generation, we developed spectrophotometric methods enabling the measurements of concentration changes of NAD(P)H, quinones, and XTT in the same reaction mixture.

	RESULTS AND DISCUSSION

TOP ABSTRACT RESULTS AND DISCUSSION MATERIALS AND METHODS LITERATURE CITED

 

Purification of a NAD(P)H Oxidoreductase Activity from Solubilized Plasma Membranes

A plasma membrane fraction showing NADH-dependent XTT reduction in the presence of MD and detergent was isolated from the upper hypocotyl region of dark-grown soybean seedlings by established techniques and checked for contaminating proteins (see "Materials and Methods"). Extensive washing of the membranes with 1.5 M NaCl or CaCl₂ did not affect this activity (data not shown). The proteins solubilized from these membranes by Tween 20 were subjected to affinity chromatography on a Blue Sepharose column. Extensive washing with buffer removed the bulk of the nonbound proteins, including a FeCN reductase, from the bound XTT-reducing fraction that could be eluted from the column with 1 µM NADH (Fig. 1A ). The protein concentration of the active enzyme fraction was very low (4–8 µg mL^–1). The elution profile obtained with the active enzyme fraction after chromatography on a calibrated Superdex 200 column revealed a single peak of an apparent molecular mass of approximately 85 kD (Fig. 1B). Redox activities of this enzyme fraction in the absence and presence of MD in comparison with the solubilized plasma membrane are summarized in Table I .

View larger version (23K): [in this window] [in a new window] [as a PowerPoint slide]   Figure 1. Purification of a MD-dependent NAD(P)H oxidoreductase activity by chromatography on Blue Sepharose (A) and Superdex (B). A, A sample of 5 mL of solubilized plasma membrane extract was applied to a 16- x 1-cm column of Blue Sepharose Fast Flow equilibrated with 10 mM HEPES (pH 8.0) containing 0.2% (w/w) Tween 20. The column was washed (0.5 mL min–1) with 100 mL of the same buffer (fractions 0–107), followed by gradient elution (0–5 µM NADH; fractions 108–167) and 1 M NaCl (fractions 168–200) in the same buffer. B, A sample of 0.7 mL of enzyme purified as shown above (fractions 110–120) together with a small amount of vitamin B12 was applied to a Superdex 200 HR 10/30 column, eluted (6 mL h–1) with 10 mM HEPES (pH 8.0), and collected in 300-µL fractions. The column was calibrated with Cyt c (12.4 kD), myoglobin (17.8 kD), chymotrypsin (25 kD), ovalbumin (43 kD), bovine serum albumin (67 kD), aldolase (160 kD), catalase (230 kD), and ferritin (440 kD) as shown in the inset. The position of the oxidoreductase is indicated by dashed lines.

This reaction is suppressed by the disproportionation of O₂^·– with SOD.

View larger version (15K): [in this window] [in a new window] [as a PowerPoint slide]   Figure 2. Consumption of O2 by the NAD(P)H oxidoreductase, its suppression by XTT, and the partial reversion of the suppression by SOD (pH 7.5). The addition of NADPH (200 µM), MD (100 µM), enzyme, XTT (100 µM), and SOD (100 µg mL–1) is indicated by arrows. The measurements were performed in a 2-mL total volume containing 1.3 µg mL–1 purified enzyme.

Peroxidase Activity of the Purified Plasma Membranes

The formation and decomposition of reactive oxygen species is affected by peroxidases. Moreover, hydroquinones can be converted into semiquinones by these enzymes (Ohnishi et al., 1969). Plasma membranes isolated from maize roots were reported to contain at least two tightly bound guaiacol peroxidases (Mika and Lüthje, 2003). We tested aliquots (50 µg of protein) of our solubilized plasma membrane fraction with the assay used by these authors and found no detectable peroxidase activity. Using a tetramethylbenzidine-based assay with increased sensitivity revealed a peroxidase activity of 12 nmol min^–1 mL^–1 (6 nmol min^–1 mg^–1 protein), corresponding to 1.7 ng of horseradish peroxidase equivalents per milligram of protein estimated from a standard curve with pure horseradish peroxidase. The peroxidase activity solubilized from the plasma membrane accounted for 0.06% of the soluble peroxidase activity in the tissue homogenate, indicating that significant amounts of peroxidases appear not to be obligatory components of plant plasma membranes.

Effects of Oxidoreductase Inhibitors

We investigated the effect of several diagnostic inhibitors on the NAD(P)H-oxidizing and XTT-reducing activities of the enzyme purified from plasma membranes to compare them with known classes of oxidoreductases. The data summarized in Figure 3 demonstrate that: (1) KCN and NaN₃ (10 mM) had no effect on XTT reduction; (2) Zn²⁺ and Cd²⁺ inhibited XTT reduction only at very high concentrations (50% inhibitory concentration [I₅₀] = 2 mM and 5 mM, respectively); (3) DPI (500 µM) had no effect on both assay reactions; (4) Cibacron Blue and dicumarol inhibited both assay reactions (I₅₀ = 3–5 µM and 300 µM, respectively); and (5) Cu²⁺ and Mn²⁺ inhibited XTT reduction but not NADPH oxidation (I₅₀ = 1 µM and 100 µM, respectively), indicating that these redox-active ions interfered with the electron transfer from the reduced MD to XTT rather than with the initial catalytic activity of the enzyme.

View larger version (15K): [in this window] [in a new window] [as a PowerPoint slide]   Figure 3. Effects of various inhibitors on the NAD(P)H oxidoreductase activity, measured either as oxidation of NADPH (200 µM; white symbols, dashed lines) or reduction of XTT (100 µM; black symbols) in the presence of MD (100 µM) at pH 7.5. NADPH oxidation was measured in the absence of XTT. Reaction mixtures with dicumarol and DPI contained up to 2% dimethyl sulfoxide, which had no effect on enzyme activity (100% = 4 µM min–1 produced by 1.3 µg mL–1 purified enzyme).

An important result emerging from this list deserves further consideration, namely the insensitivity of the enzyme to DPI, an inhibitor inactivating many flavoenzymes, including NOX-type enzymes at less than 10 µM (Cross, 1987; Doussiere and Vignais, 1992). DPI binds to, and thereby inactivates, the catalytic center of these enzymes only after its reduction to the phenyl radical (O'Donnell et al., 1994); therefore, it attacks specifically one-electron-transferring flavoenzymes such as NOX (Cross, 1987) or mitochondrial NADH:ubiquinone reductase (Ragan and Bloxham, 1977). As a consequence, flavoenzymes transferring two electrons in one step from NAD(P)H to various acceptors are not subject to inhibition by DPI (Cross, 1987). Examples of this class are the NAD(P)H:quinone-acceptor oxidoreductases known as DT-diaphorases in animals (Lind et al., 1990; Ross, 1997). Functionally related flavoenzymes have also been found in plants (Spitsberg and Coscia, 1982; Luster and Buckhout, 1989; Valenti et al., 1990; Serrano et al., 1994; Rescigno et al., 1995; Trost et al., 1995, 1997; Sparla et al., 1996, 1998). These enzymes catalyze the transfer of a hydride atom to various benzoquinones and naphthoquinones, directly forming the corresponding hydroquinones and thus avoiding the intermediate semiquinone radical that can reduce O₂ to O₂^·– (Iyanagi and Yamazaki, 1970; Lind et al., 1990; Sparla et al., 1996; Ross, 1997). A purified quinone oxidoreductase investigated by Trost et al. (1997) was shown to be insensitive to DPI. A further remarkable feature of this group of enzymes is that they can be inhibited by Cibacron Blue (Prestera et al., 1992) and dicumarol (Lüthje et al., 1994; Rescigno et al., 1995).

Evidently, the enzyme isolated from soybean plasma membranes shares some important properties with two-electron-transferring quinone reductases. Therefore, the basic problem is to explain the ability of this enzyme to elicit one-electron transfer from NAD(P)H, presumably via quinone intermediates, to O₂, a property that appears to be incompatible with the reaction mechanism of DPI-insensitive NAD(P)H oxidoreductases.

Catalytic Properties of NAD(P)H Oxidoreductase

The following experiments were conducted with the purified enzyme fraction eluted from Blue Sepharose by NADH (Fig. 1A). Table II shows the kinetic parameters for the substrates involved in the O₂-reducing reaction measured by the XTT assay. In order to elucidate the role of quinones, we examined the ability of several NQs and 1,4-benzoquinones (BQs) to replace MD in this reaction (Table III ). Unsubstituted NQ, 5-hydroxy-NQ, and 5-hydroxy,2-methyl-NQ supported XTT reduction similar to MD. The enzyme was inactive with 2-hydroxy- and 2-methoxy-substituted NQs as well as phylloquinone and menaquinone-4. Only those NQs that can be reduced by NADPH to the respective hydroquinones supported XTT reduction. However, the accumulation of hydroquinones fell short of NADPH consumption to an extent depending on the type of NQ. XTT reduction in the presence of active NQs could only partially be inhibited by removing O₂^·– with a saturating amount of SOD, and again this depended on the particular NQ. None of the tested BQs supported XTT reduction, although several of them were reduced by NADPH to the corresponding hydroquinones that accumulated in stoichiometric amounts. This result is in conflict with the reaction catalyzed by one-electron-transferring reductases that includes the intermediary formation of semiquinone.

In order to clarify the connections between NADPH oxidation and O₂^·– production, we examined the stoichiometries between NADPH oxidation, O₂ consumption, and XTT reduction in the MD-mediated reaction system (Fig. 4 ). If all electrons delivered by NADPH are utilized for the reduction of O₂ to O₂^·– (NADPH + 2 O₂ NADP⁺ + H⁺ + 2 O₂^·–), the molar ratio of NADPH oxidation to O₂ consumption would be 1:2. If the disproportionation of O₂^·– into H₂O₂ (2 O₂^·– + 2 H⁺ H₂O₂ + O₂) is taken into account, the ratio will be 1:1. Figure 4, A and B, shows that after a lag of about 20 s, the steady-state rates of these changes show a ratio of 1:0.7, indicating that at the air-saturated O₂ concentration (260 µM) about two-thirds of the electrons removed from NADPH are utilized for reducing O₂. The O₂ consumption could be reduced by half with catalase, indicating that H₂O₂ is produced that decomposes according to H₂O₂ H₂O + O₂ (Fig. 4A). About one-third of the electrons removed from NADPH are utilized for accumulating menadionehydroquinone (MDH₂). This portion can be significantly increased by reducing the O₂ concentration in the reaction mixture from 260 µM to about 10 µM (Fig. 4B), suggesting that MDH₂ accumulation competes with O₂ reduction for electrons. (For technical reasons, it was not possible to establish O₂ concentrations lower than 10 µM during the reaction.) If XTT was added to the reaction mixture, it captured the electrons removed from NADPH with a molar ratio that varied between 1:1 and 1:0.7 in different experiments at both air-saturated and reduced O₂ concentrations (Fig. 4C). This correlation presumably reflects a variable contribution of MDH₂ accumulation that in turn is influenced by the rate of the enzyme reaction. Similar to XTT, Cyt c was able to capture most of the electrons removed from NADPH (molar ratio of 1:1.7, in good agreement with NADPH + 2 Cyt c_oxidized NADP⁺ + H⁺ + 2 Cyt c_reduced; Fig. 4D).

View larger version (11K): [in this window] [in a new window] [as a PowerPoint slide]   Figure 4. Concentration changes of various substrates involved in the transfer of electrons from NADPH to XTT or Cyt c in the reaction catalyzed by the NAD(P)H oxidoreductase (200 µM NADPH and 100 µM MD, pH 7.5). A, O2 consumption with and without catalase (200 µg mL–1). B, MD reduction and simultaneously measured NADPH oxidation at 260 µM O2 (aerobic) or about 10 µM O2 (anaerobic). C, Reduction of added XTT (100 µM) and simultaneously measured NADPH oxidation under aerobic or anaerobic conditions. D, Reduction of added Cyt c (50 µM) and simultaneously measured NADPH oxidation under aerobic or anaerobic conditions.

View larger version (11K): [in this window] [in a new window] [as a PowerPoint slide]   Figure 5. pH dependence of NADPH oxidation and XTT reduction affected by the NAD(P)H oxidoreductase in the presence of MD. Experimental details are as described for Figure 4, except that the pH was adjusted by mixing 20 mM HEPES and 20 mM MES. NADPH oxidation was measured in the absence of XTT; however, similar results were obtained in the presence of XTT.

View larger version (15K): [in this window] [in a new window] [as a PowerPoint slide]   Figure 6. NADPH oxidation, MDH2 accumulation, O2 consumption, and XTT reduction affected by the NAD(P)H oxidoreductase at pH 6. Experimental details are as described for Figure 4, except that the reaction mixture was adjusted to pH 6.0 with MES.

Two genetically unrelated families of two-electron-transferring NAD(P)H:quinone-acceptor oxidoreductases have been identified in plants. Both contain FMN and are based on subunits of similar size. The enzyme cloned from Arabidopsis, AtNQR [for Arabidopsis NAD(P)H:quinone-acceptor oxidoreductase], by Sparla et al. (1999) belongs to a family of tetrameric flavoproteins composed of 21- to 22-kD subunits (Trost et al., 1995, 1997; Sparla et al., 1998). The NAD(P)H:quinone-acceptor reductase cloned from Arabidopsis, AtFQR1, by Laskowski et al. (2002) belongs to the WrbA family of flavoproteins that show sequence similarities to flavodoxins and other prokaryotic and fungal proteins. These enzymes are dimers or tetramers of 21-kD subunits (Patridge and Ferry, 2006).

To test whether the NAD(P)H oxidoreductase purified from soybean plasma membranes was related to one of these families, we examined its affinity to antibodies raised against recombinant AtNQR and AtFQR1. Native PAGE of cytosolic proteins, solubilized plasma membranes, and purified oxidoreductase revealed similar bands for MD-dependent O₂^·–-producing activity using nitroblue tetrazolium chloride (NBT) in-gel staining (Fig. 7A ). Immunoblots of these gels demonstrated that the activity purified from the plasma membranes can be attributed to NQR (Fig. 7B), while the activity in the cytosolic fraction can be attributed to FQR1 (Fig. 7C). For unknown reasons, the activity in the plasma membrane fraction showed only a very weak signal with the NQR antibody. When similar samples were subjected to SDS-PAGE, no clear protein bands could be detected by silver staining in the purified enzyme preparation (Fig. 8 ). Only faint bands at 60, 80 to 90, and 110 kD became visible, indicating the presence of impurities. NQRs are characterized by an extraordinarily high specific activity and, as such, the protein associated with the catalytic activity has been reported to be difficult to detect (Trost et al., 1997). Immunoblots of the SDS gels showed a single band at approximately 22 kD, similar to recombinant AtNQR, with the antibody against NQR but not with the antibody against FQR1 in the purified oxidoreductase preparation. On the other hand, the FQR1 antibody gave a positive reaction with a cytosolic antigen of very similar size (Fig. 8).

View larger version (70K): [in this window] [in a new window] [as a PowerPoint slide]   Figure 7. Native PAGE and immunoblot analysis of protein fractions containing cytosolic proteins (lane 1), solubilized plasma membrane proteins (lane 2), and purified NAD(P)H oxidoreductase protein (lane 3). Amounts of samples giving the same activity of XTT reduction (10 nmol XTTH2 min–1 for A and 30 nmol XTTH2 min–1 for B and C) were loaded on the gel. A, The gel was stained for enzyme activity using the NBT assay. B and C, Immunoblots were decorated with antibodies directed against NQR and FQR1.

View larger version (49K): [in this window] [in a new window] [as a PowerPoint slide]   Figure 8. Silver-stained SDS-PAGE (8%) and immunoblot analysis of protein fractions containing cytosolic proteins (lane 1), solubilized plasma membrane proteins (lane 2), purified NAD(P)H oxidoreductase protein (lane 3), and recombinant AtNQR (1 µg; lane 4). Samples with the following activities were loaded onto the gel for silver staining: 8 nmol XTTH2 min–1 (15 µg; lanes 1 and 2) and 140 nmol XTTH2 min–1 (7.5 µg; lane 3); samples with the following activities were loaded onto the gel for blotting: 30 nmol XTTH2 min–1 (lanes 1 and 2) and 140 nmol XTTH2 min–1 (lane 3). Marker positions (kilodaltons) are given on the left side. Immunoblots were decorated with antibodies directed against NQR and FQR1. The amount of NQR protein in the plasma membrane protein fraction (lane 2) was insufficient for detectable NQR antibody binding.

Mass spectrometry (MS) analysis performed with the proteins extracted from the NBT-stained band obtained with the purified plasma membrane enzyme (Fig. 7A, lane 3) confirmed the homology with the NAD(P)H:quinone-acceptor oxidoreductase NQR (EC 1.6.5.2, formerly EC 1.6.99.2). Table V summarizes the peptides that identify a translation of the assembled EST Glycine_max-35276 being homologous with AtNQR (see also the sequence alignment provided as Supplemental Table S1). Interestingly, the NQR contains a FMN-binding site that was first identified in a FMN reductase of Pseudomonas aeruginosa by x-ray crystallography and that is clearly distinguishable from the flavodoxin key fingerprint motif (Agarwal et al., 2006). This FMN reductase shows high sequence homology with NQR. The largest quantity of the NQR peptides coincided with the center of the NBT-stained gel bands. Most of the peptides identified in the stained region of the gel were from lipoxygenase-4 (swissprot identifier P38417), which was not responsible for the NBT reduction. Other peptides detected were mainly from soybean ESTs, which were homologous with the fasciclin-like arabinogalactan proteins 1 and 2 from Arabidopsis (swissprot identifiers Q9FM65 and Q9SU13). However, the profiles of these signals did not match the profile of the NBT-staining signal (data not shown). Two weak signals in the MS spectra identify peptides of a FQR1 homolog (EST Glycine_max-394114201), but their integrated intensity was more than 30-fold smaller than that of peptides from NQR. If significant, these signals are likely due to a minor contamination with soluble proteins.

Redox Properties of MDH₂

The results reported to date indicate that the purified NQR shares many features with the two-electron-transferring DT-diaphorases of mammals (Märki and Martius, 1960; Ernster et al., 1962; Lind et al., 1990; Ross, 1997) and certain quinone reductases of plants (Luster and Buckhout, 1989; Trost et al., 1995; Sparla et al., 1999), with the notable exception of the ability to reduce O₂ to O₂^·– at pH 6.5. This reaction implies the formation of a semiquinone intermediate and the capacity for one-electron-transferring reaction (van Gestelen et al., 1998). A key to explain this seemingly disparate property emerged when we investigated the stability of MDH₂ as a function of pH. When added to buffered water containing 260 µM O₂, MDH₂ was stable at acidic pH. However, autoxidation increased steeply when the pH was raised to 6.5 (Fig. 9A ). XTT reduction was inhibited by SOD by only 50% (Fig. 9B). The molar ratios (1:1 in the case of O₂ and XTT, 1:2 in the case of Cyt c) showed that the electron transfer from MDH₂ to these acceptors was complete (Fig. 10 ). Net O₂ consumption was prevented when XTT was present (Fig. 10A), similar to the enzyme-catalyzed reaction (Fig. 2). Moreover, in agreement with the results shown in Table IV, SOD reduced the molar ratio of MDH₂ oxidation/XTT reduction from 1:1 to 1:0.5, indicating that 50% of the electrons provided by MDH₂ could be diverted to XTT without the participation of O₂^·– (Fig. 10B). In the case of Cyt c, this fraction increased to 70% (Fig. 10C).

View larger version (10K): [in this window] [in a new window] [as a PowerPoint slide]   Figure 9. MDH2 autoxidation (A) and accompanying XTT reduction in the absence and presence of SOD (B) as a function of pH. A, MDH2 (100 µM) from a freshly prepared 5 mM stock solution in ethanol was added to HEPES (20 mM) adjusted to pH 5.0 to 7.7. The decrease of A290 due to the conversion of MDH2 to MD was recorded for 1 min. At pH > 7.5, the rates were too rapid to be followed accurately. B, Similar measurements recording the reduction of XTT (100 µM) with or without SOD (100 µg mL–1) in the presence of MDH2 (100 µM).

View larger version (10K): [in this window] [in a new window] [as a PowerPoint slide]   Figure 10. Molar relations in the electron transfer from MDH2 to O2 (A), XTT (B), or Cyt c (C) at pH 7.5. A, Various amounts of MDH2 dissolved in ethanol were added to HEPES in the absence or presence of XTT (100 µM). The amounts of O2 consumed were measured when the reaction was completed (after 6–10 min). B and C, Reduction of XTT (100 µM; B) or Cyt c (100 µM; C) in the absence or presence of SOD (100 µg mL–1) measured after completion of the reaction (after 1–2 min).

View larger version (15K): [in this window] [in a new window] [as a PowerPoint slide]   Figure 11. Kinetics of the autoxidation of MDH2 (A), concomitant uptake of O2 (B), and reduction of added XTT (C) or Cyt c (D) at pH 7.5. A, Oxidation of MDH2 (100 µM) was followed (A290) in 260 µM O2 (aerobic) and about 10 µM O2 (anaerobic) in the absence or presence of SOD (100 µg mL–1). B, Decrease of O2 concentration during the oxidation of MDH2. C and D, Reduction of XTT (200 µM; C) or Cyt c (200 µM; D) added to 100 µM MDH2 aerobically or anaerobically.

Reaction Mechanisms Involved in the Oxidation of MDH₂ by O₂ or XTT

The ability of redox-labile hydroquinones to form semiquinones in alkaline solution (i.e. in their anionic form) is well known in chemistry (Brunmark and Cadenas, 1989). A general scheme illustrating the reactions involved in MDH₂ autoxidation via the semiquinone (MD^·–) intermediate state is depicted in Figure 12 . MDH₂ produced by NQR (reaction 1) and activated by deprotonation at pH 6.5 (reaction 2) can undergo conversion to MD via two routes (A and B) involving three one-electron-transferring reactions (Cadenas, 1995):

(3)

(4)

(5)

View larger version (8K): [in this window] [in a new window] [as a PowerPoint slide]   Figure 12. Redox chemistry involved in the MD-mediated univalent reduction of O2 by route A and route B. Reaction 1, Divalent enzymatic reduction of MD to MDH2 by NQR; reaction 2, activation of MDH2 by deprotonation; reaction 3, univalent oxidation of MD2–, producing MD·– (semiquinone) by reducing O2 to O2·–; reaction 4, univalent oxidation of MD2–, producing MD·– by reducing O2·– to H2O2; reaction 5, oxidation of MD·– by reducing O2 to O2·–.

(6)

Moreover, the data from Figures 10 and 11 demonstrate that XTT can replace O₂ by reacting either with MD^2– or with MD^·–:

(7)

or

(8)

Because of the negative standard redox potential of the MD^·–/MD couple (–203 mV) compared with the MD^2–/MD^·– couple (+193 mV; Öllinger et al., 1990), reaction 8 will be thermodynamically strongly favored over reaction 7. However, in either case, only 50% of the XTT will be reduced via O₂^·– (reaction 6) and route B will be shut off due to the lack of O₂^·–. This explains the finding that the overall reaction can be inhibited by 50% with SOD (compare with Table IV; Figs. 9B and 10B). The lower inhibitory effect of SOD in the case of Cyt c (Fig. 10C) could be due to the ability of this acceptor to react to some extent with both MD^2– and MD^·–. Evidently, XTT and Cyt c reduction specifically detect O₂^·– production only to the extent that can be inhibited by SOD.

The autoxidation of the hydroquinones is affected by SOD in various ways (Öllinger et al., 1990). As shown in Figure 11A, SOD causes a partial inhibition of the O₂-limited MDH₂ oxidation. The removal of O₂^·– eliminated electron flow through route B. No effect of SOD on NADPH oxidation, MDH₂ accumulation, and O₂ consumption was detected in the much slower autoxidation reaction limited by the enzymatic production of MDH₂ (Table IV), suggesting that O₂^·– had no major influence on autoxidation under these conditions.

Similar to SOD, electron acceptors such as XTT or Cyt c will decrease the concentration of O₂^·– in the reaction system, shutting down route B. Nevertheless, electron flow is strongly enhanced even at very low O₂ concentrations (Fig. 11, C and D). These results show that route A is sufficient to mediate rapid electron flow provided that suitable sinks are available to remove O₂^·– and MD^·–.

Potential Function of NQR in the Plasma Membrane of Intact Cells

Based on their biochemical properties, quinones and their reduced forms can exhibit both antioxidant and prooxidant activities. For example, linoleic acid autoxidation can be inhibited by phylloquinone and enhanced by phyllohydroquinone (Canfield et al., 1985). With respect to their biological functions in animal cells, cytosolic two-electron-transferring quinone reductases are often considered to act as antioxidant enzymes, protecting the cell against the harmful accumulation of quinones that can produce toxic radicals upon reduction by one-electron-transferring reductases (Lind et al., 1982; Cadenas, 1995; Ross, 1997). In plants, an antioxidant function of two-electron-transferring quinone reductases was recently supported by the observation that the expression of these enzymes can be upregulated in vivo under stress conditions that involve the formation of toxic oxidants (Matvienko et al., 2001; Greenshields et al., 2005). On the other hand, the supposition that these enzymes generally serve as antioxidant tools to protect against quinone toxicity has been challenged on the ground that redox-labile hydroquinones can autoxidize in vivo with the formation of reactive oxygen species, including hydroxyl radicals (Nutter et al., 1992; Dicker and Cederbaum, 1993; Cadenas, 1995). The plasma membrane plays an important role as a site of O₂^·– and H₂O₂ generation, serving functions such as cell wall expansion or pathogen defense. Although this performance is often ascribed to NOX-type enzymes (Gapper and Dolan, 2006), alternative sources of reactive oxygen species cannot be excluded. This is especially true in those cases in which O₂^·– production cannot be inhibited by even high concentrations of DPI and in which a significant part of XTT or Cyt c reduction is resistant to inhibition by SOD. Examples of striking DPI insensitivity of O₂^·– production or transmembrane electron transport by plasma membrane vesicles have been reported (Menckhoff and Lüthje, 2004; Mojovi et al., 2004). As shown here, the NQR purified from plasma membranes has a potential to elicit O₂^·– production, unaffected by DPI, if supplied with a quinone substrate such as MD. Autoxidation of the hydroquinone produced in this way can lead directly to O₂^·– and H₂O₂ formation. Alternatively, coupling of O₂^·– generation to hydroquinone oxidation could be accomplished by peroxidase at the apoplastic side of the plasma membrane. Ohnishi et al. (1969) have shown that horseradish peroxidase catalyzes the conversion of hydroquinones to semiquinone radicals in the presence of H₂O₂, even at acidic pH not permitting autoxidation. In both cases, a low-potential cytochrome as a one-electron donor for the reduction of O₂ would be unnecessary. A low-potential b-type cytochrome is an essential component of NOX enzymes but in fact has never been detected in plasma membranes of plants (Bérczi and Møller, 2000). Quinones such as ubiquinone or plastoquinone function as lipid-soluble, mobile electron carriers in mitochondrial or thylakoid membranes, suggesting a similar condition in the plasma membrane (Barr et al., 1992). Specifically, this property could be utilized to mediate an electron transport from NAD(P)H oxidation by NQR at the cytoplasmic face to O₂ reduction at the apoplastic face of the plasma membrane. In this case, only catalytic amounts of quinone would be required, which undergo redox cycling and thereby transport electrons (and protons) across the membrane, in agreement with the net equation describing the reaction catalyzed by NOX:

Basic questions arising in this context concern the access to substrates and the environmental conditions for the activity of NQR in or at the plasma membrane in vivo. These questions are still wide open. Nevertheless, several findings have been reported hinting at a redox-mediating function of quinones also in the plasma membrane (e.g. the inhibition of electron transport processes by "vitamin K antagonists" such as dicumarol; Döring et al., 1992; Lüthje et al., 1994). Although MD (vitamin K₃) is not a normal constituent of the plasma membrane, a substance with the chromatographic and spectroscopic properties of phylloquinone (menadione with a phytyl side chain, vitamin K₁) has been isolated from plasma membrane preparations of maize roots (Lüthje et al., 1998; Lochner et al., 2003). Phylloquinone serves as an electron transfer component in PSI of photosynthesis (Brettel, 1997). Unfortunately, the solubility of phylloquinone in water is extremely low, preventing a direct test of its activity as a substrate for NQR in aqueous solution (compare with Table III). The reactivity of the prenyl-menadione derivatives (vitamin K series) with DT-diaphorase in aqueous solution decreases with the length of their prenyl side chain and parallel to their insolubility in water (Märki and Martius, 1960). This suggests that in lipophilic surroundings, phylloquinone can act as a substrate for NQR. It has indeed been demonstrated that phylloquinone is easily reduced by the DT-diaphorase if it is incorporated into the membrane of liposomes and thus can transport electrons from the outside to the inside of this vesicle (Martius et al., 1975).

	MATERIALS AND METHODS

TOP ABSTRACT RESULTS AND DISCUSSION MATERIALS AND METHODS LITERATURE CITED

 

Materials

Seedlings of soybean (Glycine max ‘Jutro’) were grown on wet vermiculite in darkness for 4.5 d at 25°C. The top 2 cm of the hypocotyl was excised and used for plasma membrane preparation.

Chemicals were obtained from Merck (polyethylene glycol 6000), Sigma or Aldrich (quinones, horseradish peroxidase, Cibacron 3G-A, dicumarol, DPI, nitrofurantoin, rotenone, piericidin A, N-ethylmaleimide, 4-chloromercuribenzoate, quinacrine, and bicinchoninic acid), Amersham Bioscience (Blue Sepharose 6 Fast Flow), Pharmacia (Superdex 200 HR 10/30 column), Roche Biochemicals (Cyt c, Cu/Zn-SOD, and catalase), and Polyscience (XTT).

MDH₂ was synthesized after Fieser et al. (1939) and purified by silica gel chromatography.

Quinone stock solutions (100 mM) were prepared in dimethyl sulfoxide or ethanol (vitamins K₁ and K₂), diluted with assay buffer to 1 mM, and used within the next 2 h. Juglone solutions had to be kept in darkness to prevent disintegration. MDH₂ was dissolved in water-free ethanol and added directly to the reaction medium.

Preparation and Solubilization of Plasma Membranes

The procedure devised by Thein and Michalke (1988) was adopted with some modifications. Batches (100 g) of hypocotyl segments were homogenized with a blender in 400 mL of cold medium containing 10 mM Tris-HCl (pH 8.0), 20 mM Na₂EDTA, 300 mM NaCl, 0.5 mM phenylmethylsulfonyl fluoride, and 1 g L^–1 bovine serum albumin. After filtering the slurry through nylon cloth, a membrane fraction was isolated by differential centrifugation (30 min at 1,500g, 45 min at 100,000g, 4°C) and resuspended in 180 mL of medium (without phenylmethylsulfonyl fluoride and albumin). Intracellular membranes were precipitated by adding 0.043 g mL^–1 polyethylene glycol 6000 and stirring for 30 min on ice. After removing the precipitate by centrifugation (30 min at 1,500g, 4°C), the plasma membranes contained in the supernatant were pelleted (45 min at 100,000g, 4°C), resuspended in 3 mL of 20 mM HEPES (pH 7.8) containing 20 mM Na₂EDTA and 250 mM Suc, and stored at –70°C.

The purity of the isolated membrane fraction was ascertained by separating the proteins of the different fractions by SDS-PAGE followed by semidry blotting on polyvinylidene difluoride membranes and decoration of the membranes with specific polyclonal antibodies directed against the Rieske protein (mitochondria) and the plasma membrane P-ATPase. The plasma membrane fraction showed the strongest signal with the anti-P-ATPase antibodies and no signal with the anti-Rieske antibodies, indicating that there was no detectable contamination by mitochondrial membranes (Supplemental Fig. S1). Conventional two-phase partitioning (Larsson et al., 1994) of microsomes resulted in a plasma membrane fraction with very similar properties if tested according to these criteria.

The cytosolic protein fraction was prepared from the homogenate by removing insoluble material by centrifugation (45 min at 100,000g, 4°C).

Membrane localization of the oxidoreductase activity was tested by incubating plasma membranes in 1.5 M CaCl₂ or 1.5 M NaCl for 1 h at 4°C in 20 mM HEPES (pH 7.8), followed by washing three times with the same buffer.

Plasma membrane suspensions were solubilized by adding an equal volume of 4% (w/v) Tween 20 and incubating for 30 min at 30°C. After clearing by centrifugation (15 min at 12,000g), the enzyme solution could be stored at –70°C without loss of activity for several months. The contamination of the solubilized plasma membrane fraction with soluble proteins was estimated by measuring the activity of the cytosolic marker enzyme Glc-6-P dehydrogenase. The concentration of the Glc-6-P dehydrogenase in the membrane fraction was about 5% of the concentration expected if the membrane vesicles contained the same concentration as the cytosolic tissue fraction.

Protein Determination

The protein contents of enzyme extracts were estimated with the bicinchoninic acid procedure as described by Kaushal and Barnes (1986) using bovine serum albumin as a standard. This method provides reliable results in the presence of detergents such as Tween 20 at protein concentrations of 1 µg mL^–1.

Enzyme Assays

Photometric measurements of reaction rates at specific wavelengths allowed the determination of XTT reduction, NAD(P)H oxidation, and hydroquinone accumulation in mixtures of these components. The standard assay mixture contained 200 µM NADPH, 100 µM MD, 100 µM XTT, and enzyme extract (start of reaction) in 20 mM HEPES (pH 7.5) in a total volume of 500 µL (25°C). XTT reduction was measured at 470 nm (₄₇₀ = 24.2 mM^–1 cm^–1) or 550 nm (₅₅₀ = 9.8 mM^–1 cm^–1) for 1 to 2 min. NADPH oxidation was measured at 340 nm (₃₄₀ = 6.21 mM^–1 cm^–1) and corrected for absorbance changes caused by XTT reduction (₃₄₀ = 5.4 mM^–1 cm^–1). Absorbance changes due to MD reduction at 340 nm (₃₄₀ = –0.09 mM^–1 cm^–1) are negligible. Because of overlapping absorbance spectra, the determination of coupled NADPH oxidation and MDH₂ accumulation (in the absence of XTT) required measurements at two wavelengths (290 and 340 nm) and mathematical separation of the two partial reactions using the following formulas (1-cm cuvette):

Suitable wavelengths pairs and extinction coefficients for corresponding measurements with other quinones were determined from difference spectra (oxidized reduced) as outlined in Supplemental Appendix S1. Modifications of the standard assays are described in the figure legends.

FeCN (500 µM) reduction was measured at 420 nm (₄₂₀ = 1.02 mM^–1 cm^–1). DCPIP (30 µM) reduction was measured at 600 nm (₆₀₀ = 22.0 mM^–1 cm^–1). Cyt c (50 µM) reduction was measured at 550 nm (₅₅₀ = 21.0 mM^–1 cm^–1).

Anaerobic conditions during the enzyme reaction were obtained by evacuating the reaction mixture followed by gassing with argon. This lowered the O₂ concentration by about 96% (10 µM).

Peroxidase activity was measured at 25°C either with 8.3 mM guaiacol and 8.8 mM H₂O₂ in 50 mM citrate-NaOH at pH 5.0 (470 nm, ₄₇₀ = 26.6 mM^–1 cm^–1; Mika and Lüthje, 2003) or with 100 µM 3,3',5,5'-tetramethylbenzidine and 5 mM H₂O₂ in the same buffer at pH 4.5 (654 nm, ₆₅₄ = 39 mM^–1 cm^–1; Imberty et al., 1984). Tested with horseradish peroxidase (Sigma type VI; 300 purpurogallin units mg^–1 protein), the detection limits of these assays were 1 ng and 10 pg, respectively, in 1 mL of reaction mixture.

Oxygen consumption was measured with a Clark-type oxygen electrode using 2 mL of standard assay mixture (25°C).

PAGE and Western Blotting

SDS-PAGE was carried out in 8% polyacrylamide. Proteins were visualized by silver staining. Native PAGE was carried out using 0.1% CHAPS instead of SDS. The sample buffer contained 40 mM Tris-HCl (pH 7.8), 0.1% CHAPS, 10% glycerol, and 0.002% bromphenol blue. Samples were mixed with sample buffer in a 2:1 ratio. The running buffer contained 25 mM Tris, 1.44% Gly, and no detergent. Gels were incubated for 20 min in 50 mM Tris-HCl (pH 7.4), 0.2 mM NBT, 0.1 mM MgCl₂, and 1 mM CaCl₂ in the dark. The reaction was started after 20 min of preincubation by adding 0.2 mM NADH and 0.1 mM MD and continued for approximately 15 min.

Proteins were transferred onto nitrocellulose (SDS-PAGE) or polyvinylidene difluoride (native PAGE) membranes by semidry blotting using a Multiphor II Novablot unit (Amersham Bioscience). For detection, the ECL system (Amersham Bioscience) was used according to the manufacturer's protocol.

Protein Identification by HPLC-Electrospray Mass Spectrometry

The NBT-stained region of a native PAGE gel derived from a sample of purified plasma membrane oxidoreductase (Fig. 7A, lane 3) was cut into 10 horizontal 2-mm strips that were processed individually to establish abundance profiles of the identified peptides. After destaining the gel slices and reduction of proteins by 10 mM 1,4-dithiothreitol, Cys residues were modified by iodoacetamide at a final concentration of 55 mM for 30 min at room temperature. After washing in 5 mM NH₄HCO₃ and dehydration by ethanol, 0.25 µg of trypsin (Promega) in 5 mM NH₄HCO₃ was added to each sample and incubated on ice for 20 min. The buffer was exchanged to 5 mM NH₄HCO₃, and digestion was done overnight at 37°C. Peptides were extracted successively with 0.1% formic acid and acetonitrile, dried, and resuspended in 3% acetonitrile and 0.1% formic acid.

Peptide mixtures were separated for nano-LC-electrospray ionization-MS/MS using a FAMOS autosampler (Dionex), an Ultimate inert HPLC system (Dionex), and an Agilent HPLC 1100 pump connected to the nano-electrospray ionization source of a Finnigan LTQ-FT (Thermo Electron Corporation) for online mass detection. Peptides were first collected on a trap column (0.1 x 15 mm, Zorbax Eclipse XDB-C18, 5 µm; Agilent Technology) for desalting and concentrating followed by separation on an analytical column made up by fused silica emitters (0.075 x 105 mm, 6 µm; Proxeon Biosystems) filled with Hydrosphere C18, 3 µm (YMC). Peptides were eluted during a 60-min gradient using 97% water, 3% acetonitrile, and 0.1% formic acid as solvent A and 80% acetonitrile, 20% water, and 0.1% formic acid as solvent B at a flow rate of 0.15 µL min^–1.

Mass spectrometric detection consisted of full scans at a resolution of 25,000 followed by data-dependent selected ion scans at a resolution of 50,000 and low-resolution MS/MS scans using a dynamic exclusion of parent ion masses for 60 s.

The MS and MS/MS spectra were searched against the soybean EST assembly from PlantGDB (Dong et al., 2005; release October 2007, based on GenBank release 161) and soybean and Arabidopsis (Arabidopsis thaliana) proteins from the uniprot database (release 12.4, October 2007) using an in-house installation of the program OMSSA (Geer et al., 2004; version 2.1). Search results were filtered and sorted using in-house-written software (F. Drepper, unpublished data). Peptide hits were considered significant if the precursor and product ion masses matched within 2 ppm and 0.5 relative mass units, respectively, and if the E-value was below 0.01.

Statistics

Data represent means or representative examples from measurements repeated three to six times. Typical SE values are shown in Figure 5 and Tables I, III, and IV but omitted in other figures for the sake of clarity.

Supplemental Data

The following materials are available in the online version of this article.

Supplemental Figure S1. Comparison of two methods of plasma membrane preparation.

Supplemental Table S1. NQR sequence alignment.

Supplemental Appendix S1. Formulas and extinction coefficients used for the determination of NAD(P)H oxidation and quinone reduction in NADPH/quinone mixtures.

	ACKNOWLEDGMENTS

 
We are grateful to K. Kienzler and B. Knapp (both Universität Freiburg) for excellent technical assistance; Dr. W. Seiche (Universität Freiburg) for synthesizing menadionehydroquinone; Drs. F. Sparla and P. Trost (Università di Bologna) for stimulating discussions and provision of NQR antibodies and AtNQR recombinant protein; and Dr. M. Laskowski (Oberlin College), Dr. W. Michalke (Universität Freiburg), and Dr. U. Schulte (Universität Düsseldorf) for providing antibodies directed against FQR1, P-ATPase, and Rieske protein, respectively. Special thanks are due to Dr. W. Haehnel (Universität Freiburg) for placing his mass spectrometry facilities at our disposal.

Received March 5, 2008; accepted April 8, 2008; published April 11, 2008.

	FOOTNOTES

 
The author responsible for distribution of materials integral to the findings presented in this article in accordance with the policy described in the Instructions for Authors (www.plantphysiol.org) is: Anja Krieger-Liszkay (anja.krieger-liszkay{at}cea.fr).

^[W] The online version of this article contains Web-only data.

www.plantphysiol.org/cgi/doi/10.1104/pp.108.118745

^* Corresponding author; e-mail anja.krieger-liszkay{at}cea.fr.

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