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Biomimetic Modeling of Copper Complexes: A Study of Enantioselective Catalytic Oxidation on -(+)-Catechin and -()-Epicatechin with Copper Complexes
The biomimetic catalytic oxidations of the dinuclear and trinuclear copper(II) complexes versus two catechols, namely, -(+)-catechin and -()-epicatechin to give the corresponding quinones are reported. The unstable quinones were trapped by the nucleophilic reagent, 3-methyl-2-benzothiazolinone hydrazone (MBTH), and have been calculated the molar absorptivities of the different quinones. The catalytic efficiency is moderate, as inferred by kinetic constants, but the complexes exhibit significant enantio-differentiating ability towards the catechols, albeit for the dinuclear complexes, this enantio-differentiating ability is lower. In all cases, the preferred enantiomeric substrate is -(+)-catechin to respect the other catechol, because of the spatial disposition of this substrate.
Reproducing complex biological reactivity within a simple synthetic molecule is a challenging endeavor with both intellectual and aesthetic goals. The sequence of examining biological reactivity, creating similar chemical architectures, and determining functional reaction conditions for model systems is a process that allows the biological code of reactivity to be deciphered. In the past years, the report on the crystal structures of type 3 copper enzymes (e.g., catechol oxidase, hemocyanins, and tyrosinase) [1–4], as too type 2-type 3 copper enzymes (e.g., ascorbate oxidase, laccase, ceruloplasmin) [5–8] has taken a new turn. The greater availability of such structural information now allows a shift in the role of synthetic modeling from structural and spectroscopic endeavors to the development of functional and catalytic models. Functional models can provide an opportunity to examine a biological reactivity at a small-molecule level of detail through systematic and comparative studies. Although one goal of modeling is reproduction of reactivity, extension of this reactivity beyond the scope of the inspiring system is perhaps an even more important objective. Adequate synthetic models that have similar structural, spectroscopic, and functional properties of active sites of copper proteins are done [9–13]. These models provide many elegant examples of selective and environmentally benign oxidants capable of performing interesting organic transformations, and many of these are copper complexes that use dioxygen as the ultimate oxidant above all in the catecholase activity [14–20]. The interest of our group has mainly focused on dinuclear, and trinuclear [21–28] copper complexes derived from octadentate nitrogen ligands which show catecholase activities. Some of these compounds contain chiral centers [24–28], and we have demonstrated the possibility to induce stereoselectivity in the catalytic oxidation of chiral catechols, such as - and -Dopa and their methyl esters. In the present paper we have extended this investigation on our chiral complexes using as substrates other potential catechols, namely, -(+)-catechin and -(–)-epicatechin, and we have found that the stereoselective catalytic oxidation of these substrates depends on the chirality of the dinuclear or trinuclear copper compounds, and on the spatial disposition of the catechols.
2.1. General Remarks
The dinuclear and trinuclear copper(II) complexes ; ; ; ; ; were prepared as described previously . The trichiral complexes and were prepared with standard procedures . The dinuclear complex was prepared as described previously . All the compounds are shown in Figure 1.
Although no problems were encountered during the preparation of perchlorate salts, suitable care should be taken when handling such potentially hazardous compounds.
2.3. Materials and Physical Methods
Commercial starting materials were used without purification and the solvents used for the reactions were all spectrophotometric grade. Acetonitrile was distilled from potassium permanganate and sodium carbonate; it was then stored over calcium hydride and distilled before use under nitrogen. The pH of the solutions was measured with an Amel instrument 338. Optical spectra were obtained with HP 8453 diode array spectrophotometer equipped with a thermostated cell holder at the temperature of C. The data were treated with the commercial program FigSys (BioSoft, Cambridge, UK). Formation kinetics was carried out under pseudo-first-order conditions at C.
2.4. Determination of Molar Absorptivities of the Quinones
It is well known that dinuclear and trinuclear model complexes, like tyrosinase, oxidizes -diphenols, triphenols, and flavonoids to quinones, but, in all cases, the resulting quinones may undergo nonenzymatic autopolymerization to produce colored compounds. To prevent further reactions of the quinones initially formed, a nucleophilic reagent, 3-methyl-2-benzothiazolinone hydrazone (MBTH), that traps the quinones and generates chromophoric adducts, was used. Unfortunately, no molar absorptivities of these adducts for the substrates were available, so a spectrophotometric method to determine the and the molar absorptivities of the adducts was performed. In general, the method is based on the oxidation of the substrate by an excess of sodium periodate, condition under which the reaction was very fast [31, 32]. The unstable quinones were trapped by the nucleophilic reagent (MBTH), and related was detected. In all the experiments, only one band developed in the range 300–900 nm, which corresponds to the adducts with MBTH. Based on the recording of , an experimental design can be carried out to determine the molar absorptivities of the different quinones, for example, performing spectra with different substrate concentrations and fitting the data so obtained to a Lambert-Beer equation by linear regression. Plots of the absorbance values obtained versus the different substrate concentrations allow calculating molar absorptivities. For -(+)-catechin (CQ), the experimental conditions were ; 50 mM phosphate buffer (pH 7.0)/MeOH (9:1, v:v) at C; 2 mM ; 1 mM MBTH; substrate concentrations (CQ) from 5 M to 40 M; quartz cell 1 cm path length; final volume in cell 2 mL. The coefficient of determination was 0.998 and the molar absorptivity was . For -(−)-epicatechin (EQ), the experimental conditions were ; 50 mM phosphate buffer (pH 7.0)/MeOH (9:1, v:v) at C; 2 mM ; 1 mM MBTH; substrate concentrations (EQ) from 5 M to 45 M; quartz cell 1 cm path length; final volume in cell 2 mL. The coefficient of determination was 0.994 and the molar absorptivity was .
2.5. Catecholase Activities
The kinetics of catalytic oxidation of -(+)-catechin and -(–)-epicatechin were studied by UV-Vis spectroscopy using a magnetically stirred and thermostated 1-cm path length cell. The temperature during the measurements was kept constant at C. A mixture of aqueous phosphate buffer (50 mM, pH 7.0)-methanol 9:1 (v:v) saturated with atmospheric oxygen was used as solvent. All the kinetic experiments were carried out in duplicate. The experiments performed over a substrate concentration range were initiated by adding a few microlitres of the complexes (final concentrations ) to the solution of the substrates; MBTH was maintained ; the concentration of the substrate was varied between and (final volume 2 mL). The formation of the stable -(+)-catechin--quinone-MBTH and -(–)-epicatechin--quinone-MBTH adducts was followed through the development of the strong absorption band at 459 nm for -(+)-catechin--quinone-MBTH, and an absorption band at 463 nm for -(–)-epicatechin--quinone-MBTH, respectively. In all the experiments, the noise was reduced by reading the absorbance difference between and 1100 nm, where the absorption remains negligible during the assay. The initial rates of oxidations were obtained by fitting the absorbance versus time curves in the first seconds of the reactions.
3. Results and Discussion
3.1. Stereoselective Catalytic Oxidations
The catalytic oxidations of catechols are the most widely employed test reaction to investigate the behavior of tyrosinase and catechol oxidase model complexes. Previous studies [24–27] have shown that chiral dinuclear and trinuclear copper complexes were able to display stereo-discriminating ability towards optically active catechols to give the corresponding -quinones. To confirm this behavior, new chiral catechols were employed in these catalytic stereoselective oxidations. -(+)-catechin and -(–)-epicatechin (flavan-3-ols) (Figure 2) constitute a class of phenolic compounds ubiquitous in plants and widely found in fruits, vegetables, and beverages [33–35]. In particular, they are one of the major quality factors in grapes and then in the resulting wine [36, 37].
The catalytic oxidation of polyphenolic substrates, including catechins, was well studied by many authors [38–41]. These reactions take place in the presence of atmospheric oxygen when polyphenol oxidase (PPO) and the corresponding substrates are mixed at the same time. The fundamental first step is the transformation of o-diphenols to the corresponding o-quinones. The fate and stability of o-quinones vary widely, depending both on the phenolic precursor and on environmental factors. In particular, the o-quinones of -(+)-catechin and -(–)-epicatechin were seen to be much less stable than those of other o-quinones. The prolonged autoxidation, either chemical or enzymic, led to the formation of polymers resulting from repeated condensation reactions between an aromatic ring of one molecule with an aromatic ring of another (“head to tail” polymerization mechanism). Depending on how phenolic compounds are oxidized, the condensation products formed from catechins may differ. In fact, the pH of the solution influences considerably the obtained products [42, 43], because at low pH values is favored the formation of colorless condensation products, whereas yellow compounds tended to be formed at higher pH values. To avoid any effect due to pH-dependence of oxidation products and to stop the reaction at quinones formation, a nucleophilic reagent MBTH, that traps the quinones and generates chromophoric adducts, was used (Scheme 1).
We have then studied the pH dependence of the reaction rates and have found that the better pH for the catalytic oxidation of catechins in the presence of the chiral copper complexes is pH 7.0. In order to make a comparison of the catalytic activity among the various chiral complexes reported here, we also studied the catalytic oxidation of the catechins in the presence of the achiral dinuclear complex and MBTH.
Assuming that, for the present biomimetic catalytic reactions, a two-step mechanism of catechol oxidation holds as in the case of our previous studies with dinuclear , and trinuclear  copper(II) complexes, the following simplified catalytic scheme can be hypothesized, where two molecules of catechol per cycle are oxidized to quinone (Q): Since, the kinetic experiments showed monophasic behavior and it was impossible to separate the two steps. Thus, either the two steps have a similar rate or the first one is slower. The dependence of the rates of the catalytic reactions as a function of the substrate concentration exhibited a hyperbolic behavior in all cases. However all the complexes exhibited substrate inhibition at high-substrate concentrations, and therefore the kinetic parameters reported in Table 1 were estimated with the equation here reported:
The copper complexes with chiral centers exhibited variable degree of stereoselectivity (Table 1) which has been evaluated using kinetic parameters with the following equation: where and are -(+)-catechin and -(–)-epicatechin.
The catalytic activity of all the complexes, except , shows that the preferred coordination of the catechols is for -(+)-catechin. This preference is probably dictated by the chirality of the binaphthyl or lysine residues, as shown by our studies on related complexes [24–26], and especially by the spatial disposition of the catechol substrates. In fact, by simple calculation of molecular energy minimization, -(+)-catechin shows a disposition almost planar with only the hydroxyl group out of plane (Figure 3(a)).
On the contrary, the -(–)-epicatechin shows a more bulky spatial structure, because the two aromatic rings are positioned on orthogonal planes, so the hindrance is very greater than in its isomeric form (Figure 3(b)).
Previous studies on the catalytic oxidations of catechol derivatives demonstrated that the reaction needs the cooperation of two close copper centers  to enable the binding of the catechol as a bridging ligand and allow a fast two-electron transfer process. In the dinuclear copper complexes, the catechin substrate can only form a productive complex by binding the catechol residue to the two copper ions in the A sites and that forces the resting part of the molecule to approach the optically active residue so that chiral recognition is possible (Scheme 2).
However, the dinuclear complexes that contain as central core the 1,1-binaphthyl residue show a rigid and bulky structure that reduces the possibility of effective chiral recognition for the catechins. In this case, the coordination of the catechols could occur on the outside of the complexes (Scheme 2, Structure II). The complex has a different design. It contains a chiral -Lysine residue as a central unit, which is much more flexible than the 1,1-binaphthyl moiety and this is connected with two arms carrying four benzimidazole donors through a pair of ortho-xylyl spacers. The high flexibility of the spacer and the length of the two arms allow a better chiral recognition of the substrates, as inferred by the kinetic constants and by the degree of stereoselectivity (Scheme 2, Structure I).
As reported in the previous papers [26, 27], the trinuclear complexes display a structure in which the Cu(II) center at B site and one of the two centers at A site are mediated by a double hydroxide bridge (Scheme 3, Structure I). In this case, the chiral recognition could depend not only on steric interactions but also by coordination of the free aliphatic hydroxide to the other Cu(II): a site (Scheme 3, Structure II) that allows a significant enantio-differentiating behavior towards optically active substrates. In fact, considering the three-dimensional structures of the two catechins reported before in Figure 3, one notices that the aliphatic hydroxide, in the -(+)-catechin, is opposite to the two catecholic groups, and therefore able to coordinate at the Cu(II) center at A site. The -(–)-epicatechin shows the aliphatic hydroxide too far from the Cu(II) center at A site and, in this case, the interaction needs a modification of the structure of the complexes with a strong tension of the ligands.
For , experimental data evidences a very low enantio-differentiation toward -(+)-catechin (see Table 1). This behavior could be due to the stacking interaction between the aromatic ring of m-xylene residue and the aromatic ring far from the catecholic one in the substrate; this interaction should be generated by a parallel disposition of the xylene and the plane of the substrate molecule.
This work was supported by the Italian Ministero dell'Università e della Ricerca (MIUR), through a Finanziamenti per l’Innovazione, la Ricerca e lo Sviluppo Tecnologico (FIRST) project.
- T. Klabunde, C. Eicken, J. C. Sacchettini, and B. Krebs, “Crystal structure of a plant catechol oxidase containing a dicopper center,” Nature Structural Biology, vol. 5, no. 12, pp. 1084–1090, 1998.
- M. E. Cuff, K. I. Miller, K. E. van Holde, and W. A. Hendrickson, “Crystal structure of a functional unit from Octopus hemocyanin,” Journal of Molecular Biology, vol. 278, no. 4, pp. 855–870, 1998.
- K. A. Magnus, B. Hazes, H. Ton-That, C. Bonaventura, J. Bonaventura, and W. G. J. Hol, “Crystallographic analysis of oxygenated and deoxygenated states of arthropod hemocyanin shows unusual differences,” Proteins: Structure, Function and Genetics, vol. 19, no. 4, pp. 302–309, 1994.
- Y. Matoba, T. Kumagai, A. Yamamoto, H. Yoshitsu, and M. Sugiyama, “Crystallographic evidence that the dinuclear copper center of tyrosinase is flexible during catalysis,” Journal of Biological Chemistry, vol. 281, no. 13, pp. 8981–8990, 2006.
- A. Messerschmidt, R. Ladenstein, R. Huber et al., “Refined crystal structure of ascorbate oxidase at 1.9 Å resolution,” Journal of Molecular Biology, vol. 224, no. 1, pp. 179–205, 1992.
- K. Piontek, M. Antorini, and T. Choinowski, “Crystal structure of a laccase from the fungus Trametes versicolor at 1.90-Å resolution containing a full complement of coppers,” Journal of Biological Chemistry, vol. 277, no. 40, pp. 37663–37669, 2002.
- N. Hakulinen, L.-L. Kiiskinen, K. Kruus et al., “Crystal structure of a laccase from Melanocarpus albomyces with an intact trinuclear copper site,” Nature Structural Biology, vol. 9, no. 8, pp. 601–605, 2002.
- I. Zaitseva, V. Zaitsev, G. Card et al., “The X-ray structure of human serum ceruloplasmin at 3.1 Å: nature of the copper centres,” Journal of Biological Inorganic Chemistry, vol. 1, no. 1, pp. 15–23, 1996.
- L. Casella and M. Gullotti, “Dioxygen activation by biomimetic dinuclear complexes,” in Bioinorganic Chemistry of Copper, K. D. Karlin and Z. Tyeklar, Eds., pp. 292–305, Chapman & Hall, New York, NY, USA, 1993.
- N. Kitajima and Y. Moro-oka, “Copper-dioxygen complexes. Inorganic and bioinorganic perspectives,” Chemical Reviews, vol. 94, no. 3, pp. 737–757, 1994.
- E. I. Solomon, U. M. Sundaram, and T. E. Machonkin, “Multicopper oxidases and oxygenases,” Chemical Reviews, vol. 96, no. 7, pp. 2563–2605, 1996.
- H.-C. Liang, M. Dahan, and K. D. Karlin, “Dioxygen-activating bio-inorganic model complexes,” Current Opinion in Chemical Biology, vol. 3, no. 2, pp. 168–175, 1999.
- V. Mahadevan, R. J. M. K. Gebbink, and T. D. P. Stack, “Biomimetic modeling of copper oxidase reactivity,” Current Opinion in Chemical Biology, vol. 4, no. 2, pp. 228–234, 2000.
- J. Manzur, A. M. Garcia, V. Rivas, A. M. Atria, J. Valenzuela, and E. Spodine, “Oxidation of 3,5-ditert-butylcatechol catalyzed by copper(II) complexes. A kinetic study,” Polyhedron, vol. 16, no. 13, pp. 2299–2305, 1997.
- M. R. Malachowski, H. B. Huynh, L. J. Tomlinson, R. S. Kelly, and J. W. Furbee J., “Comparative study of the catalytic oxidation of catechols by copper(II) complexes of tripodal ligands,” Journal of the Chemical Society, Dalton Transactions, no. 1, pp. 31–36, 1995.
- C.-H. Kao, H.-H. Wei, Y.-H. Liu, G.-H. Lee, Y. Wang, and C.-J. Lee, “Structural correlation of catecholase-like activities of oxy-bridged dinuclear copper(II) complexes,” Journal of Inorganic Biochemistry, vol. 84, no. 3-4, pp. 171–178, 2001.
- M. Gupta, P. Mathur, and R. J. Butcher, “Synthesis, crystal structure, spectral studies, and catechol oxidase activity of trigonal bipyramidal Cu(II) complexes derived from a tetradentate diamide bisbenzimidazole ligand,” Inorganic Chemistry, vol. 40, no. 5, pp. 878–885, 2001.
- P. Gentschev, N. Möller, and B. Krebs, “New functional models for catechol oxidases,” Inorganica Chimica Acta, vol. 300–302, pp. 442–452, 2000.
- C. Fernandes, A. Neves, A. J. Bortoluzzi et al., “A new dinuclear unsymmetric copper(II) complex as model for the active site of catechol oxidase,” Inorganica Chimica Acta, vol. 320, no. 1-2, pp. 12–21, 2001.
- I. A. Koval, K. Selmeczi, C. Belle et al., “Catecholase activity of a copper(II) complex with a macrocyclic ligand: unraveling catalytic mechanisms,” Chemistry—A European Journal, vol. 12, no. 23, pp. 6138–6150, 2006.
- E. Monzani, L. Quinti, A. Perotti et al., “Tyrosinase models. Synthesis, structure, catechol oxidase activity and phenol monooxygenase activity of a dinuclear copper complex derived from a triamino-pentabenzimidazole ligand,” Inorganic Chemistry, vol. 37, no. 3, pp. 553–562, 1998.
- E. Monzani, G. Battaini, A. Perotti et al., “Mechanistic, structural, and spectroscopic studies on the catecholase activity of a dinuclear copper complex by dioxygen,” Inorganic Chemistry, vol. 38, no. 23, pp. 5359–5369, 1999.
- E. Monzani, L. Casella, G. Zoppellaro et al., “Synthetic models for biological trinuclear copper clusters. Trinuclear and binuclear complexes derived from an octadentate tetraamine-tetrabenzimidazole ligand,” Inorganica Chimica Acta, vol. 282, no. 2, pp. 180–192, 1998.
- L. Santagostini, M. Gullotti, R. Pagliarin, E. Monzani, and L. Casella, “Enantio-differentiating catalytic oxidation by a biomimetic trinuclear copper complex containing L-histidine residues,” Chemical Communications, vol. 9, no. 17, pp. 2186–2187, 2003.
- M. C. Mimmi, M. Gullotti, L. Santagostini et al., “Stereoselective catalytic oxidations of biomimetic copper complexes with a chiral trinucleating ligand derived from 1,1-binaphthalene,” Journal of Molecular Catalysis A, vol. 204-205, pp. 381–389, 2003.
- M. C. Mimmi, M. Gullotti, L. Santagostini et al., “Models for biological trinuclear copper clusters. Characterization and enantioselective catalytic oxidation of catechols by the copper(II) complexes of a chiral ligand derived from (S)-()-1,-binaphthyl-2,-diamine,” Dalton Transactions, no. 14, pp. 2192–2201, 2004.
- M. Gullotti, L. Santagostini, R. Pagliarin, A. Granata, and L. Casella, “Synthesis and characterization of new chiral octadentate nitrogen ligands and related copper(II) complexes as catalysts for stereoselective oxidation of catechols,” Journal of Molecular Catalysis A, vol. 235, no. 1-2, pp. 271–284, 2005.
- G. Battaini, A. Granata, E. Monzani, M. Gullotti, and L. Casella, “Biomimetic oxidations by dinuclear and trinuclear copper complexes,” in Advances in Inorganic Chemistry, Volume 58, R. van Eldik and J. Reedijk, Eds., pp. 185–233, Academic Press, New York, NY, USA, 2006.
- F. G. Mutti, M. Gullotti, L. Santagostini et al., “Biomimetic Modelling of Copper Enzymes: Synthesis, Characterization, EPR Analysis and Enantioselective Catalytic Oxidations by a New Chiral Trinuclear Copper(II) Complex,” submitted to European Journal of Inorganic Chemistry.
- L. Casella, O. Carugo, M. Gullotti, S. Garofani, and P. Zanello, “Hemocyanin and tyrosinase models. Synthesis, azide binding, and electrochemistry of dinuclear copper(II) complexes with poly(benzimidazole) ligands modeling the met forms of the proteins,” Inorganic Chemistry, vol. 32, no. 10, pp. 2056–2067, 1993.
- S. W. Weidman and E. T. Kaiser, “The mechanism of the periodate oxidation of aromatic systems. III. A kinetic study of the periodate oxidation of catechol,” Journal of the American Chemical Society, vol. 88, no. 24, pp. 5820–5827, 1966.
- J. L. Muñoz, F. García-Molina, R. Varón, J. N. Rodriguez-Lopez, F. García-Cánovas, and J. Tudela, “Calculating molar absorptivities for quinones: application to the measurement of tyrosinase activity,” Analytical Biochemistry, vol. 351, no. 1, pp. 128–138, 2006.
- S. M. MacManus, “The handbook of natural flavonoids, volumes 1 and 2 J. B. Harborne and H. Baxter (editors), Wiley, Chichester, 1999, volume 1: xii+889 pp., volume 2: xvi+879 pp., ISBN 0-471-95893-X, £950.00 (the pair),” Talanta, vol. 54, no. 1, p. 207, 2001.
- F. C. Richard-Forget, M.-A. Rouet-Mayer, P. M. Goupy, J. Philippon, and J. J. Nicolas, “Oxidation of chlorogenic acid, catechins, and 4-methylcatechol in model solutions by apple polyphenol oxidase,” Journal of Agricultural and Food Chemistry, vol. 40, no. 11, pp. 2114–2122, 1992.
- I. C. W. Arts, B. van de Putte, and P. C. H. Hollman, “Catechin contents of foods commonly consumed in The Netherlands. 2. Tea, wine, fruit juices, and chocolate milk,” Journal of Agricultural and Food Chemistry, vol. 48, no. 5, pp. 1752–1757, 2000.
- M. Monagas, C. Gómez-Cordovés, B. Bartolomé, O. Laureano, and J. M. Ricardo da Silva, “Monomeric, oligomeric, and polymeric flavan-3-ol composition of wines and grapes from Vitis vinifera L. cv. Graciano, Tempranillo, and Cabernet Sauvignon,” Journal of Agricultural and Food Chemistry, vol. 51, no. 22, pp. 6475–6481, 2003.
- S. Pérez-Magariño and M. L. González-San José, “Evolution of flavanols, anthocyanins, and their derivatives during the aging of red wines elaborated from grapes harvested at different stages of ripening,” Journal of Agricultural and Food Chemistry, vol. 52, no. 5, pp. 1181–1189, 2004.
- J. Oszmianski and C. Y. Lee, “Enzymatic oxidative reaction of catechin and chlorogenic acid in a model system,” Journal of Agricultural and Food Chemistry, vol. 38, no. 5, pp. 1202–1204, 1990.
- S. Guyot, J. Vercauteren, and V. Cheynier, “Structural determination of colourless and yellow dimers resulting from (+)-catechin coupling catalysed by grape polyphenoloxidase,” Phytochemistry, vol. 42, no. 5, pp. 1279–1288, 1996.
- F. C. Richard-Forget and F. A. Gauillard, “Oxidation of chlorogenic acid, catechins, and 4-methylcatechol in model solutions by combinations of pear (Pyrus communis cv. Williams) polyphenol oxidase and peroxidase: a possible involvement of peroxidase in enzymatic browning,” Journal of Agricultural and Food Chemistry, vol. 45, no. 7, pp. 2472–2476, 1997.
- M. López-Serrano and A. R. Barceló, “Comparative study of the products of the peroxidase-catalyzed and the polyphenoloxidase-catalyzed (+)-catechin oxidation. Their possible implications in strawberry (Fragariaananassa) browning reactions,” Journal of Agricultural and Food Chemistry, vol. 50, no. 5, pp. 1218–1224, 2002.
- S. Guyot, V. Cheynier, J.-M. Souquet, and M. Moutounet, “Influence of pH on the enzymatic oxidation of (+)-catechin in model systems,” Journal of Agricultural and Food Chemistry, vol. 43, no. 9, pp. 2458–2462, 1995.
- M. Jiménez-Atiénzar, J. Cabanes, F. Gandía-Herrero, and F. García-Carmona, “Kinetic analysis of catechin oxidation by polyphenol oxidase at neutral pH,” Biochemical and Biophysical Research Communications, vol. 319, no. 3, pp. 902–910, 2004.
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