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First published online February 1, 2008; 10.1104/pp.107.110205

Plant Physiology 146:1920-1927 (2008)
© 2008 American Society of Plant Biologists

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BIOENERGETICS AND PHOTOSYNTHESIS

In Vivo Target Sites of Nitric Oxide in Photosynthetic Electron Transport as Studied by Chlorophyll Fluorescence in Pea Leaves1,[OA]

Barnabás Wodala, Zsuzsanna Deák, Imre Vass, László Erdei, István Altorjay and Ferenc Horváth*

Department of Plant Physiology, University of Szeged, H–6701 Szeged, Hungary (B.W., L.E., F.H.); Institute of Plant Biology, Biological Research Center of the Hungarian Academy of Sciences, H–6701 Szeged, Hungary (Z.D., I.V.); and Department of Gastroenterology, Medical and Health Science Centre, University of Debrecen, H–4001 Debrecen, Hungary (I.A.)


   ABSTRACT
TOP
 ABSTRACT
RESULTS
 DISCUSSION
 CONCLUSION
 MATERIALS AND METHODS
 LITERATURE CITED
 
The role of nitric oxide (NO) in photosynthesis is poorly understood as indicated by a number of studies in this field with often conflicting results. As various NO donors may be the primary source of discrepancies, the aim of this study was to apply a set of NO donors and its scavengers, and examine the effect of exogenous NO on photosynthetic electron transport in vivo as determined by chlorophyll fluorescence of pea (Pisum sativum) leaves. Sodium nitroprusside-induced changes were shown to be mediated partly by cyanide, and S-nitroso-N-acetylpenicillinamine provided low yields of NO. However, the effects of S-nitrosoglutathione are inferred exclusively by NO, which made it an ideal choice for this study. QA– reoxidation kinetics show that NO slows down electron transfer between QA and QB, and inhibits charge recombination reactions of QA– with the S2 state of the water-oxidizing complex in photosystem II. Consistent with these results, chlorophyll fluorescence induction suggests that NO also inhibits steady-state photochemical and nonphotochemical quenching processes. NO also appears to modulate reaction-center-associated nonphotochemical quenching.

Plants, as well as animals, respond to ambient levels of nitric oxide (NO), and also generate NO themselves via various enzymatic and nonenzymatic pathways (Yamasaki, 2000Go; Neill et al., 2003Go; Río et al., 2004Go). Indeed, in the past years, a growing amount of research has provided evidence for the multiple physiological roles of this gaseous free radical in plants (for review, see Wendehenne et al., 2004Go; Delledonne, 2005Go). The turnover of NO depends on its concentration, the ambient redox status, and the concentration of target molecules. In biological systems, NO is capable of targeting thiol- and metal-containing proteins (Lamattina et al., 2003Go). Photosynthetic and mitochondrial electron transport chains are abundant in transition metal-containing complexes, and NO and its derivative peroxynitrite are known to inhibit the mitochondrial electron transport chain (Millar and Day, 1996Go; Yamasaki et al., 2001Go). Yet, the effect of exogenous NO on photosynthetic activity in intact leaves has so far been poorly addressed, with often conflicting results.

Previous research suggests that NO gas decreases net photosynthesis rates in oat (Avena sativa) and alfalfa (Medicago sativa) leaves (Hill and Bennett, 1970Go). Lum et al. (2005)Go have identified a number of intracellular targets of NO signalization including mitochondria, peroxisomes, and chloroplasts. They found that the NO donor sodium nitroprusside (SNP) decreases the amount of Rubisco activase and the β-subunit of the Rubisco subunit-binding protein in mung bean (Phaseolus aureus).

NO is also able to influence the photosynthetic electron transport chain directly. An important action site of NO is PSII. Electron paramagnetic resonance and chlorophyll fluorescence measurements using NO gas treatment of isolated thylakoid membrane complexes have clearly demonstrated that NO can reversibly bind to several sites in PSII and inhibit electron transfer. Important binding sites of NO within the PSII complex are the nonheme iron between QA and QB binding sites (Diner and Petrouleas, 1990Go), the YD· Tyr residue of the D2 protein (Sanakis et al., 1997Go), and the manganese (Mn) cluster of the water-oxidizing complex (Schansker et al., 2002Go).

Takahashi and Yamasaki (2002)Go showed that the NO donor S-nitroso-N-acetylpenicillinamine (SNAP) does not modify the maximal quantum efficiency (Fv/Fm), but inhibits the linear electron transport rate, {Delta}pH formation across the thylakoid membrane, and decreases the rate of ATP synthesis. Yang et al. (2004)Go measured the chlorophyll fluorescence of intact potato (Solanum tuberosum) leaves treated with SNP, but did not observe any differences in {Delta}pH-dependent nonphotochemical quenching (NPQ). They found, however, that SNP decreases Fv/Fm values in a concentration-dependent manner.

The aim of this work was to resolve previous contradictory results concerning the effect of exogenous NO on photosynthetic electron transport in intact leaves using three different NO donors. We show that S-nitrosoglutathione (GSNO) is the most suitable to study the effect of NO on photosynthetic electron transport, as SNP-induced changes are mediated partly by cyanide (CN–), the by-product of its degradation; and SNAP shows modest effects due to its low yields of NO under our experimental conditions. Using GSNO, target sites of NO at both the donor and acceptor sides of PSII are identified.


   RESULTS
TOP
 ABSTRACT
 RESULTS
DISCUSSION
 CONCLUSION
 MATERIALS AND METHODS
 LITERATURE CITED
 

NO Donor Molecules Release Different Amounts of NO

Excised pea (Pisum sativum) leaf discs were incubated in covered, but not sealed petri dishes with NO donor and scavenger solutions for 2 h under 150 µmol m–2 s–1 white light. These conditions provided homogenous light treatment, thus avoiding potential illumination-related differences in chlorophyll fluorescence parameters.

Using a NO electrode, the concentration of NO released by the photochemical degradation of NO donors was determined after 2 h incubation under 150 µmol m–2 s–1 white light (Table I ). One millimolar GSNO produced the highest NO concentration with values above 2.5 µM, while 1 mM SNP and 1 mM SNAP solutions contained less than 1 µM NO. The potassium salt of 2-phenil-4,4,5,5-tetramethylimidazoline-1-oxyl-3-oxide (PTIO) successfully scavenged almost all NO released by GSNO and SNP; and hemoglobin (Hb), another NO scavenger, also eliminated considerable amounts of GSNO-derived NO. Monitoring the NO emission of NO donor solutions reveals that SNAP releases the bulk of its NO content in the first hour of the incubation, leading to residual amounts of NO after 2 h, while SNP and GSNO both yield significant amounts of NO even after 2 h illumination (data not shown). This trend is comparable with previous results on NO release kinetics from these NO donors (Floryszak-Wieczorek et al., 2006Go), and is consistent with earlier reports on the shorter half-life of SNAP (Feelisch, 1998Go).


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  		Table I. Concentration of NO (µM) generated by various NO donors

Concentration of NO generated by photolytic decomposition of NO donors at the end of a 2-h white light treatment. One-micromolar aqueous solutions of SNP, GSNO, and SNAP were assayed, and PTIO and Hb scavengers were used in concentrations of 1 mM and 4 mg mL–1, respectively. Light intensity was 150 µmol m–2 s–1. Values represent means ± SD (n = 4).

 
In accordance with the small NO concentration in 1 mM SNAP solution after 2 h incubation, 1 mM SNAP caused no significant changes in either QA– reoxidation kinetics, or chlorophyll fluorescence parameters (data not shown); therefore, SNAP is an unsuitable NO donor under our conditions.

SNP, on the other hand, produced larger amounts of NO after 2 h incubation, and significantly altered chlorophyll fluorescence parameters. Fv/Fm and photochemical quenching (qP) values of leaf discs incubated for 2 h at 150 µmol m–2 s–1 in 200 µM SNP decreased from 0.82 to 0.53 and from 0.87 to 0.39, respectively, in agreement with Yang et al. (2004)Go. However, the interpretation of SNP-mediated effects is challenging because SNP releases CN– as well as nitrosonium cation during its photolysis (Feelisch, 1998Go; Lum et al., 2005Go). It has previously been reported that CN– affects Fv/Fm (Jones et al., 1999Go) and may well affect additional chlorophyll fluorescence parameters, because CN– is known to inhibit photosynthesis at various levels. At submilimolar concentrations, CN– inhibits Rubisco (Wishnick and Lane, 1969Go) and ascorbate peroxidase (Forti and Gerola, 1977Go), leading to hydrogen peroxide accumulation, which interacts with the light activation of Calvin cycle enzymes (Kaiser, 1979Go). CN– also hinders electron transfer in PSII by competing with bicarbonate at the QAFe2+QB complex (Goussias et al., 2002Go). Indeed, applying 1 mM PTIO only partially restored the SNP-induced changes in Fv/Fm and qP values: to 0.68 and 0.63, respectively, which suggests that CN– and NO are both responsible for the effect of SNP. To provide direct evidence for a CN– effect, 200 µM SNP was substituted with 1 mM potassium CN–, as SNP may release up to five CN– molecules per SNP molecule (Friederich and Butterworth, 1995Go). Fv/Fm and qP values of leaf discs treated with 1 mM CN– decreased to 0.73 and 0.69, respectively, which is strikingly similar to results obtained in the presence of 200 µM SNP and 1 mM PTIO. Therefore, SNP is also a highly unsuitable NO donor for studies on photosynthesis.

Besides NO release, the photolysis of GSNO yields oxidized glutathione (GSSG), which may influence chlorophyll fluorescence parameters. GSSG potentially interferes with redox signaling processes in the chloroplast, such as the ferredoxine-thioredoxin pathway involved in the regulation of carbon fixation enzymes (Michelet et al., 2005Go). In addition, reduced glutathione has been shown to interfere with the NPQ mechanism by inhibiting violaxanthin deepoxidation, although the inhibition is weak, as reduced glutathione caused no significant inhibition at 2.5 mM (Xu et al., 2000Go). Michelet et al. (2005)Go have shown that 5 h incubation with 5 mM GSSG leads to glutathionylation of thioredoxin f, a key factor in the regulation of carbon fixation enzymes, which impairs light activation of the Calvin cycle, and such an effect may lead to altered chlorophyll fluorescence parameters. To rule out the possibility of a potential GSSG effect, we measured chlorophyll fluorescence parameters of leaf discs incubated for 2 h under 150 µmol m–2 s–1 white light in petri dishes containing 0.5 mM GSSG, but found no effect (data not shown).

In aqueous solutions, NO may rapidly react with water and oxygen to form nitrite (NO2–) and nitrate anions (Takahashi and Yamasaki, 2002Go). NO can also react with oxygen in the air and form nitrogen dioxide, a well-known photosynthetic inhibitor (Yamasaki, 2000Go) whose toxic effects are probably mediated by NO2–, as nitrogen dioxide forms NO2– when entering aqueous solutions (Wellburn, 1990Go). Incubating leaf discs for 2 h in a mixture of 200 µM sodium nitrite and sodium nitrate showed no effects on the examined photosynthetic parameters (data not shown). This finding rules out the possibility of effects mediated by degradation products of NO under our conditions.


NO Causes Donor and Acceptor Side Inhibition of PSII Electron Transport in Vivo

To investigate the inhibitory effect of NO on donor and acceptor side electron transfer, we measured QA– reoxidation kinetics of leaf discs incubated in a solution containing GSNO with or without the specific NO scavenger PTIO. A short saturating light pulse reduces QA, causing a rapid increase in fluorescence yield, followed by a decay in the subsequent dark period due to QA– reoxidation. Curves from untreated samples are characterized by a fast (approximately 800 µs), middle (approximately 190 ms), and a slow (approximately 10 s) phase (Fig. 1 ). GSNO caused no significant changes in either the time constants ({tau}) or the amplitude values (A) of the fast phase in accordance with Diner and Petrouleas (1990)Go, who observed inhibition after the second flash only. In the middle phase, 1 mM GSNO increased the time constants to approximately 430 ms. In the presence of the specific NO scavenger PTIO, this increase is reduced to 310 ms (Table II ). GSNO increased the amplitude of the middle phase, but the addition of PTIO led only to a minor reversal of this effect. The slower time constant of the middle phase suggests that NO inhibits the binding of plastoquinone (PQ) molecules at the QB binding site, while the increasing amplitude indicates a reduced amount of QB binding sites occupied by PQ at the time of the flash following the NO donor treatment.


Figure 1
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  		Figure 1. The effect of NO on fluorescence decay kinetics. Measurements were carried out on leaf discs that were incubated for 2 h under 150 µmol m–2 s–1 white light in distilled water (circles), 1 mM GSNO (squares), then dark adapted for 15 min with (black symbols) or without (white symbols) incubation in 100 µM DCMU. Curves are normalized to the same amplitude and each trace is the average of four measurements.

 

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  		Table II. Decay kinetics of flash-induced variable fluorescence

Analysis of the fluorescence relaxation kinetics. Measurements were performed on leaf discs, as in Figure 1, that were incubated for 2 h under 150 µmol m–2 s–1 white light in distilled water (control), or solutions containing NO donor and scavenger chemicals, each used in 1 mM concentration, then dark adapted for 15 min with or without incubation in 100 µM DCMU. The curves were analyzed in terms of two exponential components (fast and middle phases) and one hyperbolic component (slow phase). Values in parentheses are relative amplitudes as a percentage of total variable fluorescence. SEs of the calculated parameters are also indicated.

 
When QA– reoxidation via forward electron transport is inhibited by 3-(3,4-dichlorophenyl)-1,1-dimethylurea (DCMU), which occupies the QB binding site, the fast and middle phases of the fluorescence decay curve are converted to a slow phase with approximately 2 s time constant, which reflects QA– reoxidation via charge recombination with the S2 state of the water-oxidizing complex. In the presence of DCMU, a significant fraction of fluorescence does not decay in the GSNO-treated leaf discs (Fig. 1). This effect is largely prevented in the presence of PTIO (Table II). The increase in the nondecaying part of fluorescence correlates with previous results of Schansker et al. (2002)Go showing that NO reduces the Mn cluster of the water-oxidizing complex into the S-2 state. Our measurements with GSNO indicate that QA– is unable to recombine with the S2 state, possibly because NO inactivates or reduces the Mn cluster.


Fluorescence Induction Kinetics Indicates Donor and Acceptor Side Inhibition of PSII

Effects of NO on donor and acceptor side of PSII were further investigated by fluorescence induction measurements. Following incubation with GSNO, leaf discs were dark adapted, then a Kautsky curve was measured in which chlorophyll fluorescence yield rises from a minimal level (F0) through a local minimum (FI) to a peak value (FP; Lichtenthaler, 1992Go). GSNO treatment caused a 2-fold FI increase, indicating inhibition of forward electron transfer at the acceptor side of PSII due to a growing fraction of centers that could only reduce QB slowly. FP decreased to 43% of the control value, but no significant changes were observed in F0 (Fig. 2 ). The maximal slope of the FI-FP curve was also decreased by GSNO, and this effect was largely restored by the addition of 4 mg mL–1 Hb (Table III ). The decrease of FP and the slope of the FI-FP curve indicate inhibition of electron transport at the donor side of PSII.


Figure 2
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  		Figure 2. The effect of NO on fluorescence induction kinetics. Leaf discs were incubated for 2 h under 150 µmol m–2 s–1 white light in distilled water (Control), 1 mM GSNO, and 1 mM GSNO + 4 mg mL–1 Hb, then dark adapted for 15 min. Following this treatment, chlorophyll fluorescence of leaf discs was induced by 3 s of 130 µmol m–2 s–1 red light. Curves show the average of five measurements each.

 

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  		Table III. Fast fluorescence induction parameters

Fast fluorescence induction parameters of curves in Figure 3. Leaf discs were incubated for 2 h under 150 µmol m–2 s–1 white light in distilled water (control), 1 mM GSNO, and 1 mM GSNO + 4 mg mL–1 Hb, then dark adapted for 15 min. Following this treatment, chlorophyll fluorescence of leaf discs was induced by 3 s of 130 µmol m–2 s–1 red light. The F0, FI-F0, and FP-F0 parameters are shown in arbitrary units. Values represent means ± SD (n = 5).

 

Figure 3
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  		Figure 3. The effect of GSNO on Fv/Fm and on steady-state qP. Prior to measurements, leaf discs were incubated for 2 h under 150 µmol m–2 s–1 white light in distilled water (Control) and 1 mM GSNO solution, then dark adapted for 15 min. The NO scavenger Hb was applied at a concentration of 4 mg mL–1. Steady-state qP values were recorded at the end of a 30-min 130 µmol m–2 s–1 red actinic illumination. Bars represent means ± SD (n = 4). Asterisks indicate levels of significance: P < 0.05 (*) and P < 0.01 (**).

 

Effect of NO on Chlorophyll Fluorescence Parameters

Following the 2-h incubation in 1 mM GSNO with or without Hb, Fv/Fm, steady-state qP, and NPQ parameters were determined. GSNO reduced Fv/Fm and qP values, which were restored in the presence of Hb (Fig. 3 ). The results are in good correlation with fluorescence decay kinetics measurements, which indicate an accumulation of the reduced form of the electron acceptor QA–.

The rate of light-dependent acidification of the lumen depends on the rate of electron transport and also on the activity of ATP synthase. The NO-derived inhibition of linear electron transport should reduce proton accumulation in the lumen, which would then cause a decrease in NPQ via the energy-dependent quenching (qE) component. GSNO decreased steady-state NPQ, as well as qE and photoinhibitory quenching components in a concentration-dependent manner (Fig. 4 ), and this effect is eliminated by Hb. Besides decreasing steady-state NPQ, GSNO changed the length and amplitude of an NPQ transient (Fig. 5A ), which resembles the reaction-center NPQ described by Finazzi et al. (2004)Go in barley (Hordeum vulgare) leaves. Figure 5B shows the linear correlation between the increase of the amplitude of NPQ transients and the decrease in the effective quantum efficiency ({Phi}PSII) in response to growing concentrations of GSNO, which indicates that an increasing proportion of reaction centers switch from photochemistry to heat dissipation.


Figure 4
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  		Figure 4. The effect of GSNO on steady-state NPQ. Prior to measurements, leaf discs were incubated for 2 h under 150 µmol m–2 s–1 white light in distilled water (Control) and GSNO solutions with different concentrations, then dark adapted for 15 min. Hb was applied at a concentration of 4 mg mL–1. Steady-state NPQ values were recorded at the end of a 30-min 130 µmol m–2 s–1 red actinic illumination. Bars represent means ± SD (n = 4). Asterisks indicate levels of significance: P < 0.05 (*) and P < 0.01 (**).

 

Figure 5
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  		Figure 5. The effect of GSNO on NPQ transient. Prior to measurements, leaf discs were incubated for 2 h under 150 µmol m–2 s–1 white light in distilled water (Control), and 500 and 1,000 µM GSNO solutions, then dark adapted for 15 min. Hb was applied at a concentration of 4 mg mL–1. During measurements, leaf discs were illuminated with 130 µmol m–2 s–1 red actinic light. Data are presented as mean ± SD (n = 4). A, Time-dependent change of NPQ. B, Relationship between the amplitude of NPQ and the corresponding effective quantum efficiency values.

 

   DISCUSSION
TOP
 ABSTRACT
 RESULTS
 DISCUSSION
CONCLUSION
 MATERIALS AND METHODS
 LITERATURE CITED
 

The Choice of NO Donor for Chlorophyll Fluorescence Measurements in Vivo

The use of NO donors is a general tool for investigating the biological roles of NO, but the diverse chemical properties of donors potentially lead to differences in NO yield and the release of other reactive agents. These factors, together with difficulties of direct measurement of NO, may well account for the differences reported in the amounts of NO released by specific NO donors (Delledonne, et al., 1998Go, 2001Go; Lum et al., 2005Go). Our direct NO measurements clearly demonstrate the differences in NO production of SNAP, GSNO, and SNP (Table I). Measuring leaf discs treated with CN–, or SNP with or without PTIO shows that SNP releases CN–, which modifies the chlorophyll fluorescence parameters. The low NO yield of SNAP, and CN– emission of SNP make both NO donors unsuitable for our studies. On the other hand, our experiments demonstrate that the effects caused by GSNO are inferred by NO exclusively.


NO Hinders Electron Transfer in PSII in Vivo

The terminal electron acceptor in PSII is the linear QAFe2+QB complex, where QA and QB can take up one and two electrons, respectively. The rate of electron transfer between the two quinones depends on the coordinative properties of the nonheme iron (II) that, under normal circumstances, forms coordinate covalent bonds with four His residues provided by the D1 and D2 reaction center subunits, as well as one bicarbonate occupying one of the remaining two coordination places (Petrouleas and Diner, 1990Go; Kern et al., 2005Go). NO and other small molecules, such as CN– and fluoride anions, compete with bicarbonate and bind reversibly to the nonheme iron (II) (Goussias et al., 2002Go). Experiments with isolated thylakoids indicate that NO binding slows down the rate of electron transfer between QA and QB (Diner and Petrouleas, 1990Go). Binding of NO to the QAFe2+QB complex is facilitated in the presence of reduced QA– acceptor, as this reduction weakens the bond between bicarbonate and iron (Goussias et al., 2002Go). The rate of electron transport may decrease on the donor side as well, since in vitro experiments have proven that NO interacts with the YD· Tyr residue and the water-oxidizing complex. The latter is reduced to the S–2 state by NO, as shown by oxygen electrode, fluorescence, and electron paramagnetic resonance measurements (Schansker et al., 2002Go).

Our QA– reoxidation measurements show a reduced rate of electron transport between QA and QB upon NO donor treatment. This result provides circumstantial evidence in support for the competitive binding of NO to the nonheme iron in vivo (Fig. 1; Table II). Measurements in the presence of DCMU show NO induced inhibition of QA– recombination with the S2 state of the water-oxidizing complex. This donor side inhibition of electron transport may sufficiently be accounted for by the reduction of either the water-oxidizing complex, or the YD· residue by NO. Fast chlorophyll fluorescence induction kinetics of GSNO-treated leaf discs confirm significant donor and acceptor side inhibition of electron transport (Fig. 2; Table III).


Effects of NO on Chlorophyll Fluorescence Parameters

Previous chlorophyll fluorescence studies have provided controversial results on changes induced by NO. In isolated chloroplasts, NO derived from SNAP did not affect Fv/Fm; while in intact leaves, SNP-derived NO decreased its values considerably (Takahashi and Yamasaki, 2002Go; Yang et al., 2004Go). However, in both cases, the NO donor treatment caused a decrease in {Phi}PSII, which is related to qP changes. Our measurements indicate that the different chemical properties of NO donors and different experimental conditions jointly account for previous conflicting results. GSNO caused a significant decrease in Fv/Fm values in intact leaves and decreased steady-state qP, which indicates that NO increases the proportion of closed PSII reaction centers (Fig. 3). Taken together, these data provide strong in vivo evidence that a partial inhibition of PSII by NO is indeed the cause of impaired steady-state electron transport in vivo.

Besides reducing steady-state NPQ values, NO changes the amplitude and kinetics of an NPQ transient (Fig. 5A), which resembles reaction-center NPQ described by Finazzi et al. (2004)Go. Reaction-center NPQ arises upon the onset of illumination of dark-adapted leaves and, at low light intensities, it is relaxed rapidly after a few minutes of illumination. On the basis of its fast relaxation and {Delta}pH dependency, Finazzi et al. (2004)Go showed that reaction-center NPQ is caused by the rapid and transient overacidification of the thylakoid lumen, which is created by the immediate onset of photochemistry. In addition, they suggest that the {Delta}pH may be further increased by cyclic and pseudocyclic electron transport (Mehler reaction) and explain the relaxation of this transient form of NPQ by the activation of the carbon fixation apparatus, which decreases {Delta}pH and redox pressure. Although a potential effect of NO on Calvin cycle activation would account for changes in this NPQ transient, steady-state NPQ values below control values indicate that NO does not decrease the maximum rate of the Calvin cycle. Further investigations are therefore necessary to clarify the mechanism through which NO modifies the NPQ transient.


   CONCLUSION
TOP
 ABSTRACT
 RESULTS
 DISCUSSION
 CONCLUSION
MATERIALS AND METHODS
 LITERATURE CITED
 
In conclusion, this study tested an array of NO donors and scavenger chemicals on intact leaves and demonstrated that the SNP-induced changes are mediated partly by CN– and that a 2-h incubation leads to low NO yields from SNAP, while the biological effect of GSNO is related to NO exclusively. This underlines the importance of data interpretation and adequate choice of NO donor, and justifies the use of GSNO to study the effect of NO on photosynthetic electron transport in vivo. Measurements with GSNO provide in vivo confirmation of target sites of NO in PSII and further evidence on the inhibitory effect of NO on photosynthetic electron transport in intact leaves. In addition, NO was shown to modulate reaction-center-associated NPQ. Taken together, these findings confirm previous in vitro data and offer promising perspectives for NO as a potential regulator of photosynthetic electron transport yet to be discovered.


   MATERIALS AND METHODS
TOP
 ABSTRACT
 RESULTS
 DISCUSSION
 CONCLUSION
 MATERIALS AND METHODS
LITERATURE CITED
 

Chemicals

The NO donors GSNO, SNP, and SNAP were purchased from Sigma-Aldrich. The NO scavengers Hb and the potassium salt of PTIO were purchased from Sigma-Aldrich. The electron transport inhibitor DCMU was purchased from ICN Biomedicals Inc. Standard chemicals of analytical grade were from Sigma-Aldrich.


Plant Material and Experimental Solutions

Sterilized seeds of pea (Pisum sativum ‘Petit Provençal’) were germinated for 3 d at 24°C, and the seedlings were grown in a semicontrolled growth chamber for 2 weeks under a 12-h-light (150 µmol m–2 s–1)/12-h-dark cycle and temperature of 22°C. Leaf discs of the youngest fully expanded leaves were prepared by a 15 mm diameter leaf punch and used for each measurement. Prior to measurements, leaf discs were individually incubated for 2 h under 150 µmol m–2 s–1 white light in covered petri dishes, which were 10 mm deep and 36 mm in diameter, then dark adapted for 15 min. During the incubation, leaf discs were floating in the covered but not sealed petri dishes containing 4 mL of distilled water as control, or 4 mL of different dilutions of NO donor molecules and scavenger chemicals in aqueous solution. The volume of the aqueous phase left an approximately 6 cm3 upper ambient space in the covered petri dishes.

GSNO, SNP, and SNAP were used as NO donors, and Hb and PTIO were applied as NO scavengers. Some measurements were conducted in the presence of 100 µM DCMU. To increase their stability, thus preventing an early and unwanted NO release, SNP, SNAP, and GSNO stock solutions were prepared daily and kept in dark on ice until the start of experiments (Singh et al., 1996Go; Feelisch, 1998Go).


NO Measurements

Solutions of NO donors with or without scavengers were incubated in petri dishes in the same way as leaf discs, and the amount of NO released at the end of the 2-h incubation under 150 µmol m–2 s–1 white light was measured using a NO electrode (ISO-NOP; World Precision Instruments Inc.) dipped in the stirred aqueous phase. The NO electrode was calibrated by adding different volumes of SNAP solution to copper(II) sulfate solution set to pH 4 by addition of sulfuric acid following the manufacturer's instructions.


Variable Chlorophyll Fluorescence Measurements

Fluorescence Relaxation Kinetics
Flash-induced increase and the subsequent decay of chlorophyll fluorescence yield were measured by a double-modulation fluorometer (PSI) according to the method of Vass et al. (1999)Go. The instrument contained red LEDs for both actinic (20 µs) and measuring (2.5 µs) flashes, and was used in the 150-µs to 100-s time range with pea leaf discs.

Analysis of the fluorescence relaxation kinetics was based on the widely used model of the two-electron gate (Crofts and Wraight, 1983Go; Diner, 1998Go). According to this model, the fast (few hundred microsecond) decay component reflects QA– reoxidation via forward electron transport in centers, which contain bound PQ (in the oxidized or semireduced form) at the QB site before the flash. The middle (few millisecond) phase arises from QA– reoxidation in centers, which had an empty QB site at the time of the flash and have to bind a PQ molecule from the PQ pool. Finally, the slow (few second) phase reflects QA– reoxidation with the S2 state of the water-oxidizing complex, thus causing backward electron transport via the QA–QB {leftrightarrow} QAQB– equilibrium. In certain cases a nondecaying fluorescence component is also observed, which arises from PSII centers in which QA– has very stable or no recombination partner at the donor side. Since the relationship between fluorescence yield and the amount of QA– is not linear, the relative QA– concentration was estimated with Joliot's model (Joliot and Joliot, 1964Go), in which the value of the parameter for energy transfer between PSII units is 0.5. The fast and middle phases are generally described by exponential components. In contrast, the slow decay of QA– via charge recombination has been shown to obey hyperbolic decay kinetics corresponding to an apparent second-order process (Vass et al., 1999Go). Consequently, multicomponent deconvolution of the measured curves was performed by using a fitting function with two exponential components and one hyperbolic component:

Formula
where Fv, corr is the variable fluorescence yield corrected for nonlinearity, A0 to A3 are amplitudes, and {tau}1 to {tau}3 are time constants from which the half-lifetimes can be calculated as t1/2 = ln 2{tau} for the exponential components, and t1/2 = {tau} for the hyperbolic component.

Slow Fluorescence Induction Measurements
PSII chlorophyll fluorescence of pea leaves was monitored with a PAM fluorometer (PAM-2000; Heinz Walz GmbH). After the 2-h incubation, leaf discs were dark adapted for at least 15 min for precise determination of minimal and maximal fluorescence levels in the dark (Fo and Fm, respectively).

Fm was obtained by exposing the leaf sample to a high intensity (8,000 µmol m–2 s–1) short pulse (0.8 s). Fv/Fm (Fm – Fo/Fm) was calculated according to Genty et al. (1989)Go. Maximum fluorescence values in the light adapted state (Fm') were determined at the end of a 30-min actinic light illumination of 130 µmol m–2 s–1. After switching the actinic light off, far-red light was applied to determine the minimal level of fluorescence at steady state (Fo'). Steady-state qP ({Delta}F/Fm' – Fo') was determined according to the method described by Schreiber et al. (1986)Go where {Delta}F equals Fm' – Fs and Fs is the steady-state fluorescence yield during actinic illumination. {Phi}PSII ({Delta}F/Fm') was determined according to Genty et al. (1989)Go. Steady-state NPQ was calculated as: NPQ = (Fm – Fm')/Fm' (Bilger and Björkman, 1990Go).

The relaxation kinetics of steady-state NPQ was monitored by applying saturating pulses with 60-s intervals from the end of the 30-min actinic illumination period to determine the qE component of NPQ. qE relaxes in the first 5 min of the dark relaxation period and was calculated according to Thiele and Krause (1994)Go as: qE = Fm/Fm' – Fm/Fm'', where Fm'' is the maximum fluorescence yield in the fifth min of dark relaxation subsequent to the illumination period.


   ACKNOWLEDGMENTS
 
We thank Dr. Irma Tari for discussion and critical reading of the manuscript.

Received October 1, 2007; accepted January 23, 2008; published February 1, 2008.


   FOOTNOTES
 
1 This work was supported by the Hungarian Scientific Research Fund (grant nos. OTKA F 048787 and OTKA T 048436), the National Research and Development Programme (grant no. NKFP 3A/009/2004), the Economic Competitiveness Operative Programme (grant no. GVOP–3.2.1–2004–04–0419/3.0), the Poland and Hungary Action for Restructuring of the Economy (grant no. PHARE HU2003/005.830.01–04), and the European Union (grant no. MRTN–CT–2003–505069). Back

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: Ferenc Horváth (horvathf{at}bio.u-szeged.hu).

[OA] Open Access articles can be viewed online without a subscription. Back

www.plantphysiol.org/cgi/doi/10.1104/pp.107.110205

* Corresponding author; e-mail horvathf{at}bio.u-szeged.hu.


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TOP
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