# Nitration Transforms a Sensitive Peroxiredoxin 2 into a More Active and Robust Peroxidase

Lía M Randall, Bruno Manta, Martín Hugo, Magdalena Gil, Carlos

Batthyàny, Madia Trujillo, Leslie B Poole, Ana Denicola

► To cite this version:

Lía M Randall, Bruno Manta, Martín Hugo, Magdalena Gil, Carlos Batthyàny, et al. Nitration Transforms a Sensitive Peroxiredoxin 2 into a More Active and Robust Peroxidase. Journal of Biological Chemistry, 2014, 289 (22), pp.15536 - 15543. 10.1074/jbc.m113.539213. hal-05052233

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# Nitration Transforms a Sensitive Peroxiredoxin 2 into a More Active and Robust Peroxidase*

Received for publication, November 28, 2013, and in revised form, March 31, 2014 Published, JBC Papers in Press, April 9, 2014, DOI 10.1074/jbc.M113.539213

Lía M. Randall<sup>†§<fnref n="1" /></sup>, Bruno Manta<sup>†¶<fnref n="1" />,<fnref n="2" /></sup>, Martín Hugo<sup>§||<fnref n="2" /></sup>, Magdalena Gil<sup>**††</sup>, Carlos Batthyàny<sup>§||**</sup>, Madia Trujillo<sup>§||</sup>, Leslie B. Poole<sup>§§</sup>, and Ana Denicola<sup>‡§<fnref n="3" /></sup>

From the <sup>†</sup>Laboratorio de Fisicoquímica Biológica, Instituto de Química Biológica, Facultad de Ciencias, Universidad de la República, 11400 Montevideo, Uruguay, the <sup>§</sup>Center for Free Radical and Biomedical Research, Facultad de Medicina, Universidad de la República, Montevideo 11100, Uruguay, the <sup>¶</sup>Laboratorio de Biología Redox de Tripanosomas, Institut Pasteur de Montevideo, 11400 Montevideo, Uruguay, the <sup>||</sup>Departamento de Bioquímica, Facultad de Medicina, Universidad de la República, 11100 Montevideo, Uruguay, the <sup>**</sup>Unidad de Bioquímica y Proteómica Analíticas, Institut Pasteur de Montevideo, 11400 Montevideo, Uruguay, the <sup>‡</sup>Unidad de Bioquímica y Proteómica Analíticas, Instituto de Investigaciones Biológicas Clemente Estable, Ministerio de Educación y Cultura, 11600 Montevideo, Uruguay, and the <sup>§§</sup>Department of Biochemistry, Wake Forest School of Medicine, Winston-Salem, North Carolina 27157

**Background:** Peroxiredoxin 2 (Prx2) reduces peroxides through a cysteine-dependent mechanism and is susceptible to overoxidation of its reactive cysteine during catalysis.

**Results:** Nitration rendered a more active peroxidase, less sensitive to overoxidation.

**Conclusion:** Nitration of Prx2 favors disulfide bond formation over overoxidation.

**Significance:** Understanding the mechanisms by which post-translational modifications modify Prx2 functionality *in vitro* is crucial to evaluate potential *in vivo* consequences for redox signaling.

Peroxiredoxins (Prx) are efficient thiol-dependent peroxi-
dases and key players in the mechanism of H₂O₂-induced redox
signaling. Any structural change that could affect their redox
state, oligomeric structure, and/or interaction with other pro-
teins could have a significant impact on the cascade of signaling
events. Several post-translational modifications have been
reported to modulate Prx activity. One of these, overoxidation
of the peroxidatic cysteine to the sulfinic derivative, inactivates
the enzyme and has been proposed as a mechanism of H₂O₂
accumulation in redox signaling (the floodgate hypothesis).
Nitration of Prx has been reported *in vitro* as well as *in vivo*; in
particular, nitrated Prx2 was identified in brains of Alzheimer
disease patients. In this work we characterize Prx2 tyrosine
nitration, a post-translational modification on a noncatalytic
residue that increases its peroxidase activity and its resistance to
overoxidation. Mass spectrometry analysis revealed that treat-
ment of disulfide-oxidized Prx2 with excess peroxynitrite ren-
ders mainly mononitrated and dinitrated species. Tyrosine 193
of the YF motif at the C terminus, associated with the suscepti-
bility toward overoxidation of eukaryotic Prx, was identified as
nitrated and is most likely responsible for the protection of the
peroxidatic cysteine against oxidative inactivation. Kinetic ana-
lyses suggest that tyrosine nitration facilitates the intermolecular

disulfide formation, transforming a sensitive Prx into a robust
one. Thus, tyrosine nitration appears as another mechanism to
modulate these enzymes in the complex network of redox
signaling.

Peroxiredoxins (Prx,<fnref n="4" /> EC 1.11.1.15) are a group of enzymes
that efficiently reduce peroxides based on a critical cysteine
residue (peroxidatic cysteine, C<sub>p</sub>). The first step in catalysis is
the reaction of C<sub>p</sub> with H<sub>2</sub>O<sub>2</sub> to form a sulfenic acid derivative
(C<sub>p</sub>-SOH) which, in 2-cysteine Prx (2-Cys Prx), reacts with
another cysteine residue (the resolving cysteine, C<sub>R</sub>) to form a
disulfide that is then reduced by the thioredoxin/thioredoxin
reductase/NADPH system (Fig. 1) (1–4). In typical 2-Cys Prx or
Prx1 subfamily (Prx 1–4 in mammals (5)), the reaction occurs
between the C<sub>p</sub>-SOH of one subunit with the C<sub>R</sub>-SH of another
subunit; thus, each homodimer contains two active sites (3). In
addition, for the intermolecular disulfide to be formed, a con-
formational change is needed to approach the C<sub>p</sub>-SOH from
one subunit toward the C<sub>R</sub> from the other subunit. This rear-
rangement involves the transition from the so-called fully
folded (FF) form, in which the C<sub>p</sub> and the C<sub>R</sub> are approximately
14 Å apart, to a locally unfolded (LU) conformation (Fig. 1) (2, 7,
8). The sulfenic acid intermediate can react with the C<sub>R</sub>-SH
forming a disulfide, or with a second molecule of H<sub>2</sub>O<sub>2</sub> to form
sulfinic acid (overoxidation), inactivating the peroxidase activ-

<footnote>* This work was supported, in whole or in part, by National Institutes of Health Grant GM050389 (to L. B. P.). This work was also supported by Comisión Sectorial de Investigación Científica UdelaR Grant CSIC C007-348 (to A. D.) and Agencia Nacional de Investigación e Innovación Grants FCE_2011_1_S706 (to M. T.) and FCE_2007_217 (to B. M.).</footnote>

<footnote n="1">¹ Supported by Comisión Académica de Posgrados, UdelaR, and PEDECIBA (Programa de Desarrollo de las Ciencias Básicas).</footnote>

<footnote n="2">² Supported in part by the Agencia Nacional de Investigación e Innovación.</footnote>

<footnote n="3">³ To whom correspondence should be addressed: Laboratorio de Fisicoquímica Biológica, Instituto de Química Biológica, Facultad de Ciencias, Universidad de la República, Iguá 4225, 11400, Montevideo, Uruguay. Tel./Fax: 598-2-525-0749; E-mail: denicola@fcien.edu.uy.</footnote>

<footnote n="4">⁴ The abbreviations used are: Prx, peroxiredoxin(s); C<sub>p</sub>, peroxidatic cysteine; C<sub>R</sub>, resolving cysteine; C<sub>p</sub>-SOH, cysteine sulfenic acid; C<sub>p</sub>-SO<sub>2</sub>H, cysteine sulfinic acid; DTDP, 4',4'-dithiodipyridine; DTNB, 5',5'-dithio-bis(2-nitrobenzoic acid); DTPA, diethylenetriaminepentaacetic acid; ESI, electrospray ionization; FF, fully folded; LU, locally unfolded; NEM, N-ethylmaleimide; Prx2, peroxiredoxin 2; PTM, post-translational modification; QTOF, quadrupole time-of-flight; ROA, reverse-order addition; TR, thioredoxin reductase; Trx, thioredoxin.</footnote>
<figure><img src="image_2.png" /><figcaption>FIGURE 1. **Catalytic cycle of eukaryotic typical 2-Cys Prx.** 1, reaction of a molecule of peroxide with the C~p~ thiolate to form cysteine sulfenic acid. 2, transition from the FF to the LU conformation. 3, reaction of C~p~ sulfenic acid with C~R~. 4, reduction of disulfide Prx. 5, overoxidation of C~p~ to sulfinic acid. 6, reduction of cysteine sulfinic acid by sulfiredoxin (Srx)/ATP. The protein is represented as one of two active sites within a functional dimer.</figcaption></figure>

ity. The oxidation of cysteine to cysteine sulfinic acid (C~p~SO~2~H) is an irreversible post-translational modification (PTM) for most proteins other than 2-Cys Prx, where the specific enzymatic reduction of C~p~-SO~2~H by sulfiredoxin in an ATP-dependent mechanism was demonstrated (9, 10).

Prx are ubiquitous and highly expressed proteins, and their extraordinary reactivity and specificity for hydroperoxides make them ideal sensors of endogenous H~2~O~2~ and probably the first step in H~2~O~2~-induced signaling pathways (11–15). PTM of Prx that could affect their activity, redox state, oligomeric structure, or interaction with other proteins will undoubtedly affect redox signaling by H~2~O~2~, and it has been hypothesized that Prx inactivation via overoxidation is a way to accumulate H~2~O~2~ to allow oxidation of other redox proteins (the floodgate hypothesis) (2). The presence of sulfiredoxin as an enzyme that specifically reduces typical 2-Cys Prx cysteine sulfinic acid supports the biological relevance of their peroxidase activity and the signaling role of their oxidative inactivation (16).

Prx2, the most abundant peroxidase in mammalian erythrocytes (17, 18), is capable of reducing hydroperoxides as well as peroxynitrite,<fnref n="5" /> a potent oxidant formed *in vivo* by the diffusion-controlled reaction between superoxide and nitric oxide. Our group recently demonstrated that erythrocyte Prx2 not only is susceptible to overoxidation by peroxynitrite, but it can also get nitrated during catalysis (19). Moreover, nitrated Prx2 was detected in brains of patients with early Alzheimer disease (20).

Protein tyrosine nitration is a common PTM occurring under conditions of nitroxidative stress, which alters the structure and function of the modified protein. The biological mechanism of tyrosine oxidation begins with the formation of the tyrosyl radical followed by addition of nitrogen dioxide yielding 3-nitrotyrosine, and one of the major pathways of protein nitration *in vivo* involves the reaction of radicals derived from peroxynitrite homolysis (21–25).

We herein report the effects of Prx2 modification by peroxynitrite treatment, focusing on tyrosine nitration, which increases its peroxidase activity along with resistance to overoxidation by H~2~O~2~. We hypothesize that nitration of tyrosine 193 from the YF motif at the C terminus, close to the active site,

favors transition from the FF to the LU conformation, promoting disulfide formation and inhibiting C~p~ overoxidation.

## EXPERIMENTAL PROCEDURES

*Chemicals*—Dithiothreitol (DTT), DTNB, and reduced nicotinamide adenine dinucleotide phosphate (NADPH) were purchased from AppliChem (Germany). DTDP was purchased from ACROS Organics, Fisher Scientific. Hydrogen peroxide (H~2~O~2~) and DTPA were purchased from Sigma. Peroxynitrite was synthesized as in Ref. 26. All other reagents were of analytical grade and used as received.

*Purification of Proteins*—Human Prx2 was purified from human erythrocytes according to Ref. 19. Recombinant human thioredoxin (hTrx1), *Escherichia coli* thioredoxin 1 (*EcTrx1*), and recombinant *E. coli* thioredoxin reductase (*EcTR*) were produced and purified as reported in Refs. 19 and 27. *Echino-coccus granulosus* (*EgTR*) was kindly provided by Dr. G. Salinas (28).

*Peroxide and Protein Quantification*—The concentration of H~2~O~2~ stock solutions was measured at 240 nm (ε~240~ = 43.6 M~−~1 cm~−~1). Peroxynitrite concentration was determined at 302 nm (ε~302~ = 1670 M~−~1 cm~−~1) as in Ref. 26. Protein concentration was measured by absorption at 280 nm in the assay buffer, using the corresponding ε determined for the oxidized proteins according to Ref. 29: ε~280~(Prx2) = 19,380 M~−~1 cm~−~1, ε~280~(hTrx) = 7100 M~−~1 cm~−~1, ε~280~(*EcTrx*) = 14,060 M~−~1 cm~−~1, and ε~280~(*EcTR*) = 19,160 M~−~1 cm~−~1. Concentration of active *EgTR* was estimated according to FAD and selenium content (28).

*Thiol Quantification*—The thiol concentration of the reduced proteins was measured according to Ref. 30 with minor modifications. Briefly, the protein was reduced with DTT (>10-fold molar excess for 30 min) and the remnant reductant removed by buffer exchange with a HiTrap coupled to a FPLC with online UV detection equilibrated in 50 mM potassium phosphate buffer, pH 7.4, with 0.1 mM DTPA and 150 mM NaCl. An excess of DTDP was added to the protein sample in the assay buffer, and absorption was measured at 324 nm (ε~324~ = 21,400 M~−~1 cm~−~1).

*Prx2 Thiol Reduction and Oxidation*—For reduction of purified Prx2, the enzyme was reduced with 1 mM DTT for 30 min at room temperature immediately before the experiment, and the mixture was passed twice through a Bio-Spin column (Bio-Rad) preequilibrated with the assay buffer. Thiol concentration was determined just after elution from the column, and controlled oxidation to its disulfide form was achieved with the addition of 0.6 eq of H~2~O~2~.

*Nitration of Prx2 by Peroxynitrite*—To prevent overoxidation of C~p~, treatment with peroxynitrite was performed on the disulfide-oxidized enzyme. The corresponding molar excess of peroxynitrite was added in a unique bolus or a flux-like addition. Previously decomposed peroxynitrite in the assay buffer (reverse-order addition (ROA)) was used as a control of peroxynitrite-derived products reaction with Prx2. Tyrosine nitration of Prx2 was confirmed by Western blot analysis using specific antibodies. Briefly, samples were prepared for 15% SDS-PAGE under reducing (Figs. 2B and 4C) or nonreducing conditions (Fig. 3) without heating and transferred to a PVDF membrane. The membrane was incubated with anti-nitroty-

<footnote n="5">⁵ The term peroxynitrite is used to refer to the sum of peroxynitrite anion (ONOO⁻) and peroxynitrous acid (ONOOH) unless specified.</footnote>
Effects of Nitration on Prx2 Functionality

<figure><img src="image_3.png" /></figure>

FIGURE 2. Analysis of Prx2 nitration after peroxynitrite treatment. A, QTOF-ESI MS analysis. Disulfide-oxidized Prx2 was treated with a 5-fold excess peroxynitrite, then reduced with 5 mM DTT for 15 min at room temperature, followed by addition of 20 mM NEM to block the reduced thiols. The remaining DTT and NEM were removed by gel filtration, and samples in 30 mM ammonium bicarbonate buffer were analyzed by QTOF-ESI MS. Control Prx2 is shown in black (shown as 100%), and the gray dotted line shows the peroxynitrite-treated enzyme. B, Western blot analysis. Disulfide Prx2 was treated with a 5-fold excess peroxynitrite (ONOO⁻) or ROA. 2.4 µg of control or peroxynitrite-treated Prx2 was resolved on 15% SDS-PAGE under reducing conditions and analyzed by Western blot using α-NO₂Y antibodies.

<figure><img src="image_4.png" /></figure>

FIGURE 3. Differential overoxidation of control and peroxynitrite-treated Prx2. After treatment with the ROA control or a 5-fold excess of peroxynitrite (ONOO⁻), Prx2 was treated with DTT for reduction of its thiols, and residual DTT was removed. 5 µM Prx2 was incubated with 0, 0.01, 0.02, 0.06, 0.12, 0.24, or 5 mM H₂O₂ in 50 mM phosphate buffer, pH 7.4. After 5 min, 30 mM NEM was added to alkylate the remaining thiols. Samples were prepared for SDS-PAGE under nonreducing conditions, analyzed by Western blotting using α-Prx2 antibody and α-Cₚ-SO₂/₃H after mild stripping. One µg of protein was loaded on each lane (D<sub>ss</sub>, dimer with one Cₚ disulfide-oxidized; D<sub>ss/ssSS/SS</sub>, dimer with both Cₚ disulfide-oxidized; *M*, monomer).

rosine antibodies (α-NO₂Y (31)) in a 1/1000 dilution and with goat anti-rabbit IRDye® 800 CW (LI-COR Biosciences) secondary antibody (1/20,000).

*Overoxidation of Prx2 by H₂O₂*—To study the effect of nitration on the susceptibility of Prx2 to overoxidation, it was necessary to start with a reduced nonoveroxidized but yet nitrated form of Prx2. Disulfide-oxidized Prx2 was treated with peroxynitrite for nitration as described above, then reduced, and after removal of residual DTT the enzyme was treated with H₂O₂. Samples were resolved in 15% SDS-PAGE under nonre-

ducing conditions, transferred to a PVDF membrane, and blotted with specific α-Prx2-Cₚ-SO₂/₃H antibodies (AbFrontier). For control, rabbit polyclonal antibodies against Prx2 were used (α-Prx2; AbFrontier).

*Mild Stripping of Western Blot Membranes*—Membranes were incubated for 10-min in mild stripping buffer (1.5% glycine, 0.1% SDS, pH 2.2) twice, followed by two 10-min incubations in PBS and two 5-min incubations in TBS-Tween 0.1%. Blockage was performed for 2 h or overnight in 5% milk in TBS-Tween 0.1%.

*NADPH-linked Peroxidase Activity*—NADPH consumption was followed spectrophotometrically at 340 nm in a Cary 50 spectrophotometer (Varian). Prx2 was mixed with 120 µM NADPH, 0.4 µM *EgTR*, 8 µM hTrx1 in the described buffer, and the reaction was started with the addition of H₂O₂. An Applied Photophysics RX2000 Rapid Kinetics Spectrophotometer Accessory was used for stopped-flow experiments.

*Thioredoxin-linked Peroxidase Activity*—The catalytic H₂O₂ decomposition by Prx2 was followed through the intrinsic fluorescence (λ<sub>exc</sub> = 280 nm, λ<sub>em</sub> = 340 nm) of reduced *EcTrx1* (10 µM) in a coupled assay with Prx2 (50 nM) and H₂O₂ (7 µM) in a thermostatted Cary Eclipse spectrofluorometer (Varian). Fluorescence changes were calibrated using a known concentration of reduced and oxidized *EcTrx1*.

*MS Analysis of Prx2 Tryptic Digestion*—For analysis of proteins obtained from acrylamide gels, selected bands were manually cut and in-gel digested with trypsin (sequence grade; Pro-mega) as described (32). Peptides were extracted from gels using aqueous 60% acetonitrile containing 0.1% TFA and concentrated by vacuum drying. Mass spectra of peptides mixtures were acquired in a linear ion trap mass spectrometer (LTQ Velos, Thermo) coupled on-line with a nano-liquid chromatography system (easy-nLC; Proxeon-Thermo). Peptides were separated in a reversed-phase column (EASY-column™ C18, 75 µm × 10 cm, inner diameter) equipped with a trap column (EASY-column C18, 100 µm × 2 cm, inner diameter) with solvent A (0.1% formic acid in H₂O) and solvent B (0.1% formic acid in acetonitrile), and eluted using a linear gradient from 0 to 45% B in 70 min at 300 nl/min. Electrospray voltage was 1.6 kV, capillary temperature was 270 °C. Peptides detected in the positive ion mode using a mass range of 300–2000.

Proteins were identified by database searching of measured peptide *m/z* values using the MASCOT search engine (Matrix Science) and Sequest (Thermo) software, based on the following search parameters: monoisotopic mass tolerance, 1.5 Da; fragment mass tolerance, 0.8 Da; partial methionine oxidation, cysteine carbamidomethylation, tyrosine nitration, and three missed tryptic cleavages allowed. Protein mass and taxonomy were unrestricted. Significant scores (*p* < 0.05) were used as criteria for positive peptide identification.

*Whole Protein Mass Spectrometry Analysis of Peroxynitrite-treated Prx2*—Control and peroxynitrite-treated Prx2 were reduced, and 20 mM NEM was added to alkylate thiols. Remaining DTT and NEM were removed using Bio-Gel P6 Gel® (Bio-Rad) columns and 30 mM ammonium bicarbonate buffer for elution. Samples were diluted from 4 to 40 µl with methanol: H₂O 1:1 2% formic acid, and 2–3 µl were analyzed using a Waters Q-Tof API US operated in “V” mode using a Triversa
Nanomate sprayer from Advion. Sprayer voltage ~ 1.8 kV; Q-T of cone voltage 45 V; source temperature 80 °C; nitrogen desolvation temperature 200 °C. Data were acquired from 600–1900 *m/z* in positive ion continuum mode; scan time 2.4 s; interscan delay 0.1 s. Max Ent data were produced for 10,000–50,000 Da.

## RESULTS

**Treatment of Prx2 with Peroxynitrite Yields a Nitrated Enzyme**—Disulfide-oxidized Prx2 was treated with a 5-fold excess of peroxynitrite or its decomposition products, as a control designated ROA. Nitration of Prx2 was confirmed by inunoblotting and mass spectrometry analyses (Fig. 2). For QTOF-ESI mass spectrometry analysis, disulfide-oxidized Prx2 was reduced with DTT and alkylated with NEM. A main peak of *m/z* 22,053 was obtained for control Prx2, which corresponds to the Prx monomer (21,803 Da) with both C<sub>p</sub> and C<sub>r</sub> alkylated with NEM (125 Da) (Fig. 2A). When treated with a 5-fold excess of peroxynitrite, mainly mononitrated (*m/z* 22,053 ± 45) and dinitrated (*m/z* 22,053 ± (2 × 45)) species were detected, confirming that nitration is the main modification after peroxynitrite treatment of disulfide Prx2. The minor species detected in both experiments (*m/z* 21,959) corresponds to the monomer of Prx2 with one Cys NEM-alkylated and the other one overoxidized, suggesting initial oxidation of Prx2 with H<sub>2</sub>O<sub>2</sub> to obtain the disulfide form rendered a minor portion of overoxidized protein (Fig. 2A). Western blot analysis using antibodies against nitrotyrosine residues confirmed tyrosine nitration after the peroxynitrite treatment (Fig. 2B). Some nonreducible dimers were observed, suggesting the presence of di-tyrosine dimers, characteristic of peroxynitrite treatment of proteins (22).

**Analysis of Peroxynitrite-treated Prx2 Overoxidation**—2-Cys Prx sensitivity to overoxidation can be followed by nonreducing SDS-PAGE (33, 34). As shown in Fig. 3, and consistent with results in Fig. 2, overoxidation was detected at lower H<sub>2</sub>O<sub>2</sub> concentrations for the nontreated Prx2 than for the peroxynitrite-treated enzyme. Addition of increasing concentrations of H<sub>2</sub>O<sub>2</sub> to reduced control or peroxynitrite-treated Prx2 caused the transition from reduced monomer (M) to mono-disulfide dimer (D<sub>SS</sub>) and di-disulfide dimer (D<sub>SS/SS</sub>), with high H<sub>2</sub>O<sub>2</sub> concentrations rendering overoxidized disulfide dimer (D<sub>SS</sub>) and overoxidized monomer (M). As observed previously (33, 35), substoichiometric addition of H<sub>2</sub>O<sub>2</sub> was enough to overoxidize the enzyme in these conditions, leading to the formation of dimers containing a disulfide and an overoxidized C<sub>p</sub>, whereas high concentrations of the oxidant were not able to completely overoxidize the enzyme to its monomers. This result supports the idea of asymmetry of the homodimer active sites, suggesting that, under noncatalytic conditions, the redox state of one C<sub>p</sub> affects overoxidation of the second one, as discussed previously by others (35–38). Moreover, nitration protected Prx2 from overoxidation, as the treated enzyme showed less overoxidation after H<sub>2</sub>O<sub>2</sub> treatment than the control under noncatalytic conditions, suggesting a structural connection between tyrosine nitration and overoxidation of the peroxidatic cysteine.

## Effects of Nitration on Prx2 Functionality

<figure><img src="image_5.png" /></figure>

**FIGURE 4.** **Effect of nitration on Prx2 peroxidase activity and overoxida- tion.** A, NADPH-linked peroxidase activity. 0.5 µM reverse-order addition (●) or peroxynitrite-treated (○) Prx2 was incubated with 8 µM hTrx1, 0.4 µM EgTR, and 160 µM NADPH in 50 mM sodium phosphate buffer, pH 7.4, 150 mM NaCl, 0.1 mM DTPA. The reaction was started by the addition of H<sub>2</sub>O<sub>2</sub> (10 µM final concentration), and consumption of NADPH was followed at 340 nm. B, *EcTrx1* fluorescence-linked Prx2 peroxidase activity. Oxidation of *EcTrx1* was followed at λ<sub>exc</sub> = 280 nm, λ<sub>em</sub> = 340 nm, in 50 mM sodium phosphate buffer, pH 7.4, 0.1 mM DTPA, 150 mM NaCl, with 10 µM reduced *EcTrx1*, and 50 nM Prx2. ●, nontreated Prx2; △, Prx2 treated with 1-fold or (○) 5-fold excess peroxynitrite; ▼, control run (no Prx2 added). The reaction was started by the addition of 7 µM H<sub>2</sub>O<sub>2</sub>. C, Western blot analysis against C<sub>p</sub>-SO<sub>2/3</sub>H. Aliquots were taken at 0, 0.5, and 1 min after H<sub>2</sub>O<sub>2</sub> addition in the presence of Trx, TR, and NADPH. Catalase (0.3 mg/ml) was added to eliminate residual H<sub>2</sub>O<sub>2</sub> and NEM (26 mM) to block remaining thiols. 80 ng of Prx2 was loaded on each lane and resolved by reducing SDS-PAGE.

**Treatment of Prx2 with Peroxynitrite Affects Its Peroxidase Activity**—Peroxidase activity was measured following the consumption of NADPH at 340 nm after addition of H<sub>2</sub>O<sub>2</sub> to a system containing Prx2, hTrx1, EgTR, and NADPH (Fig. 4A). Treated Prx2 showed a higher rate of H<sub>2</sub>O<sub>2</sub> reduction than the ROA control. The gain in peroxidase activity was confirmed by following NADPH consumption in a stopped-flow spectrophotometer, demonstrating that the change in peroxidase activity precedes oxidative inactivation of the enzyme (data not shown), as well as following the loss of reduced *EcTrx1* fluorescence at 340 nm (λ<sub>exc</sub> = 280 nm) as it was oxidized by Prx2/H<sub>2</sub>O<sub>2</sub> (Fig. 4B). The inactivation during turnover was clear for the native Prx2, whereas the peroxynitrite-treated enzyme suffered less overoxidation in turnover, as indicated by Western blot analysis (Fig. 4C).
Effects of Nitration on Prx2 Functionality

Interaction of Nitrated Prx2 with hTrx1 Does Not Explain the Increase in Peroxidase Activity—To understand the gain in Prx2 peroxidase activity after treatment with peroxynitrite, we measured peroxidase activity using increasing concentrations of hTrx1 at a fixed concentration of H₂O₂ (Fig. 5). Interestingly, when low concentrations of hTrx1 were used, control and treated-Prx2 showed no clear differences in their peroxidase activity, whereas increasing hTrx1 concentrations enhanced their differences. As shown in Fig. 5, even in the presence of high concentrations of hTrx1 (>10-fold the reported K<sub>m</sub><sup>app</sup> (19)), a significant difference between untreated and peroxynitrite-treated Prx2 activity was observed. Fitting the data from Fig. 5 to the Michaelis-Menten equation, V<sub>max</sub> can be calculated, obtaining a higher value for the peroxynitrite-treated enzyme than for control Prx2.

**Mapping of the Modified Residues Reveals Nitration of Tyr-193**—Analysis of digested Prx2 in an LTQ mass spectrometer mapped four of the seven tyrosine residues of the polypeptidic chain. From these peptides, three of the residues (Tyr-33, Tyr-126, and Tyr-193) were detected as nitro-tyrosines after peroxynitrite treatment, whereas Tyr-115 was found as native in every experiment. Table 1 shows the theoretical and experimental mass values for the modified tyrosine-containing peptides detected. Among these, Tyr-193 is part of the YF motif located in the C terminus region of the protein that has been related to Prx sensitivity to overoxidation (Fig. 6) (2), and the environment of the YF loop has been recently described to have a great impact on C<sub>p</sub> overoxidation (35).

<figure><img src="image_6.png" /><figcaption>FIGURE 5. Dependence of Prx2 peroxidase activity with thioredoxin concentration. Nontreated (●) or 5-fold excess peroxynitrite-treated (○) Prx2 activity was measured following NADPH consumption at 340 nm. The reaction was started with the addition of 10 µM H₂O₂ to a mixture containing 160 µM NADPH, 0.4 µM *EgTR*, varying concentrations of hTrx1 (0.8–60 µM), and 0.5 µM Prx2.</figcaption></figure>

<caption>**TABLE 1**
Identification of modified tyrosine-containing peptides after treatment with peroxynitrite</caption>

Control and peroxynitrite-treated Prx2 were digested with trypsin after 15% SDS-PAGE. Samples were subjected to HPLC-MS/MS using an LTQ mass spectrometer as detailed under "Experimental Procedures." Sequences of modified tyrosine-containing peptides identified by MS are shown, with their corresponding theoretical and observed masses.

<table><thead><tr><th rowspan="2">Peptide</th><th>Theoretical mass</th><th>Theoretical mass + 45<sup>a</sup></th><th rowspan="2">Observed masses</th><th rowspan="2">Assigned sequence</th><th rowspan="2">Nitrated tyrosine</th></tr><tr><th>[(M + H)<sup>+</sup>]</th><th>[(M + H)<sup>+</sup>]</th></tr></thead><tbody><tr><td>1</td><td>625.3</td><td>670.3</td><td>670.2</td><td><sup>30</sup>LSD<sup>33</sup>YK<sup>34</sup></td><td>Tyr-33</td></tr><tr><td>2</td><td>673.3</td><td>718.3</td><td>718.2</td><td><sup>192</sup>E<sup>193</sup>YFSK<sup>196</sup></td><td>Tyr-193</td></tr><tr><td>3</td><td>924.4</td><td>969.4</td><td>969.3</td><td><sup>120</sup>TDEGIA<sup>126</sup>YR<sup>127</sup></td><td>Tyr-126</td></tr></tbody></table>

DISCUSSION

The peroxidatic cysteine of Prx reacts with H₂O₂ at 10³⁻ to 10⁶⁻fold faster than most protein cysteines (13), but at ordinary rates with any other thiol reagent (39). Prx seem to be designed to specifically reduce peroxides, which place them not only as efficient antioxidant enzymes but also as key players in the mechanism of H₂O₂-induced redox signaling (40, 41). The catalysis of H₂O₂ reduction depends on a conserved Cys residue within a highly conserved active site pocket that adequately stabilizes the transition state. In addition, an important conformational change is needed for 2-Cys Prx to complete the oxidative part of the cycle, including the local unfolding of the helix that harbors Cₚ and the displacement of secondary structure elements that contain the Cₘ residue (2). Stabilization of the FF form of the enzyme has been associated with a slower rate of disulfide formation favoring the reaction of Cₚ-SOH with H₂O₂ to form the inactive sulfinic derivative (Cₚ-SO₂H). This inactivation by overoxidation has been postulated as a mechanism of regulating intracellular H₂O₂ levels, critical for redox signaling (2, 14, 42–44).

MS analysis of disulfide Prx2 treated with a 5-fold excess of peroxynitrite revealed that the main polypeptidic modification was nitration of tyrosine residues yielding mainly mononitrated and dinitrated species (Fig. 2A). Nitration of Prx2 rendered an enzyme less susceptible to overoxidation by H₂O₂ (Figs. 3 and 4C). This could be due either to a slower reaction with the second H₂O₂ molecule to yield the sulfinic derivative (step 5 in Fig. 1) or to a faster formation of the intermolecular disulfide (steps 2 and 3 in Fig. 1), thus unfavoring the overoxidation reaction.

<figure><img src="image_7.png" /><figcaption>FIGURE 6. Structural model of Prx2 active site. View of human erythrocyte Prx2 active site. One monomer shows the Cₚ residue in sulfinic acid form (blue) whereas the other subunit (gray) shows the Cₘ as well as the YF motif containing Tyr-193. The image was constructed with PyMOL from PDB 1QMV (6).</figcaption></figure>

<footnote><sup>a</sup> Addition of a nitro (-NO₂) group results in a molecular mass increase of 45 Da.</footnote>
Surprisingly, the peroxynitrite-treated enzyme was more active than the native enzyme (Fig. 4). Given the modified enzyme is more resistant to overoxidation, one possible explanation for the observed gain in activity could be less inactivation in turnover (as seen in Fig. 4C). However, measurement of activity by stopped-flow spectrophotometry showed a higher rate for the nitrated enzyme from the very beginning of the run (0.277 ± 0.006 µmol/min *versus* 0.213 ± 0.002 µmol/min for the untreated enzyme; data not shown), indicating the differences in activity preceded overoxidation in turnover.

The reaction of C~P~ with H~2~O~2~, the first step in catalysis, is so fast ($k_2$ = 10^7–10^8 M⁻¹ s⁻¹) that it is safe to assume C~P~-SOH formation will not be the limiting step (19, 39). Thus, under the experimental conditions employed, the gain in peroxidase activity should reside in disulfide formation between C~P~-SOH and C~R~ and/or the reduction of the intermolecular disulfide by thioredoxin (Fig. 1). The first option will be kinetically limited by the conformational change needed to get together both cysteines (the FF-LU transition (8)) whereas the second is limited by the kinetics of protein-protein interaction (Fig. 1). As shown in Fig. 5, at a fixed saturating concentration of H~2~O~2~, initial NADPH consumption rates were very close for control and peroxynitrite-treated Prx2 at low concentrations of hTrx1, whereas a significant difference appeared at higher hTrx1 concentrations. Although a faster dissociation of the ternary complex between hTrx1 and Prx2 to yield reduced Prx2 could explain the observed differences in V~max~, it cannot explain the resistance to overoxidation of the nitrated enzyme. Therefore, it can be affirmed that, at high hTrx1 concentrations, the velocity of NADPH consumption is limited by disulfide formation. From V~max~ and Prx2 concentration, the rate constant of this step, k~cat~, can be estimated, obtaining a value of (1.2 ± 0.1) s⁻¹ for the ROA control enzyme and (1.6 ± 0.1) s⁻¹ for the peroxynitrite-treated Prx2. Very similar results were obtained when using *Ec*TR and *Ec*Trx1 (data not shown), supporting the idea that the observed changes in V~max~ are not due to differences in the interaction between Prx2 and Trx. The faster the intermolecular disulfide bond is formed, the lower the chance for C~P~ to get overoxidized by H~2~O~2~. These differences in k~cat~ explain the differences in activity as well as the different susceptibility to overoxidation. Thus, this PTM transforms a sensitive Prx into a more robust peroxidase.

It has been observed that eukaryotic Prx, generally more sensitive to overoxidation than prokaryotic Prx, present a YF motif at the C terminus (Fig. 6) that packs over the active site in the FF form of the protein and delays the conformational change that brings together C~P~ and C~R~, therefore slowing down the disulfide formation and favoring the overoxidation reaction (3, 8, 33, 35). In addition, different susceptibility toward overoxidation was found between different mammalian 2-Cys Prx isoforms. Human mitochondrial Prx3 is more resistant to this modification than cytosolic Prx2 (33). Recent work by Haynes et al. (35) demonstrated that residues near the C~R~ at the C terminus modulate the extent of C~P~ overoxidation. The substitution of residues at the C terminus of Prx3 resulted in a Prx2-like enzyme, more susceptible to overoxidation (35). Moreover, truncation of the C terminus containing the YF motif was reported to decrease overoxidation of Prx (45, 46). The YF sequence motif

in the C-terminal helix of one subunit covers helix α2 containing the C~P~ of the adjacent subunit, stabilizing the FF form, thus making difficult the unfolding of the C~P~-containing α2 to reach C~R~ (2). Tyr-193, which was nitrated by peroxynitrite treatment (Table 1) belongs to this YF motif and is most likely responsible for the resistance to overoxidation of the nitrated enzyme (Fig. 6). It is interesting to note that in *in vitro* experiments where Jurkat cell lysates were treated with peroxynitrite, the YF motif tyrosine of Prx1 was identified as nitrated (47).

Prx are key enzymes for detoxifying H~2~O~2~ as well as sensing H~2~O~2~ in redox signaling. In this context, the modulation of Prx peroxidase activity and interaction with other proteins is critical. Modification of the reactive cysteine causes inactivation of the peroxidase activity as seen for overoxidation to sulfinic/ sulfonic acid. Glutathionylation and S-nitrosation of C~P~ have also been reported (48–50). Interestingly, phosphorylation of noncatalytic residues in Prx1 and Prx2 could decrease, as well as increase, their peroxidase activity, suggesting a fine interplay between H~2~O~2~⁻ and kinase-driven signaling pathways (51–54). Similar to our results, N-acetylation of Lys-196 in Prx2 causes an increase in peroxidase activity and a decrease in overoxidation susceptibility (55). Again, modification of residues at the C terminus, adjacent to C~R~ (Lys-196, Thr-194, and Tyr-193 in this work) can affect activity and the extent of overoxidation.

Nitration of tyrosine residues has an impact on protein structure and activity (in general, inactivation, although a gain of function has also been reported) and is linked to a variety of pathological conditions such as neurodegenerative and cardiovascular diseases (56, 57). Nitration of typical 2-Cys Prx has been reported *in vitro* and *in vivo* (20, 47, 58). In particular, Prx2 was identified in a proteomic analysis as one of the nitrated brain proteins in early Alzheimer disease (20). This could have an impact on intracellular H~2~O~2~-induced signaling cascades, including Prx2-protein interactions, which still remains to be explored. Our work characterizes the nitrated form of Prx2 as a more active and robust peroxidase by favoring the intermolecular disulfide formation, placing tyrosine nitration as another mechanism of modulating Prx in the complex network of redox signaling.

Acknowledgments—We thank M. P. Samuel, M. J. Thomas, and K. J. Nelson (Wake Forest School of Medicine, Winston-Salem, NC) for assistance in samples preparation and whole protein mass spectrometry analysis; B. Alvarez and G. Ferrer-Sueta (Universidad de la República, UdelaR, Uruguay) for helpful discussions; J. Santos (Universidad de Buenos Aires, Argentina) for kindly providing *Ec*Trx1 plasmid; G. Salinas (Institut Pasteur de Montevideo, Uruguay) for the *Ec*TR protein; and L. Blixen for graphical work assistance.

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