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Chlorophyll b to Chlorophyll a Conversion Precedes Chlorophyll Degradation in Hordeum vulgare L.

1999; Elsevier BV; Volume: 274; Issue: 31 Linguagem: Inglês

10.1074/jbc.274.31.21811

1083-351X

Patrick Folly, Norbert Engel,

Light effects on plants

This study reveals by in vivodeuterium labeling that in higher plants chlorophyll (Chl)b is converted to Chl a before degradation. For this purpose, de-greening of excised green primary leaves of barley (Hordeum vulgare) was induced by permanent darkness in the presence of heavy water (80 atom % 2H). The resulting Chla catabolite in the plant extract was subjected to chemical degradation by chromic acid. 3-(2-Hydroxyethyl)-4-methyl-maleimide, the key fragment that originates from the Chl catabolite, was isolated. High resolution 1H-, 2H-NMR and mass spectroscopy unequivocally demonstrates that a fraction of this maleimide fragment consists of a mono-deuterated methyl group. These results suggest that Chl b is converted into Chla before degradation. Quantification proves that the initial ratio of Chl a:Chl b in the green plant is preserved to about 60–70% in the catabolite composition isolated from yellowing leaves. The incorporation of only one deuterium atom indicates the involvement of two distinguishable redox enzymes during the conversion. This study reveals by in vivodeuterium labeling that in higher plants chlorophyll (Chl)b is converted to Chl a before degradation. For this purpose, de-greening of excised green primary leaves of barley (Hordeum vulgare) was induced by permanent darkness in the presence of heavy water (80 atom % 2H). The resulting Chla catabolite in the plant extract was subjected to chemical degradation by chromic acid. 3-(2-Hydroxyethyl)-4-methyl-maleimide, the key fragment that originates from the Chl catabolite, was isolated. High resolution 1H-, 2H-NMR and mass spectroscopy unequivocally demonstrates that a fraction of this maleimide fragment consists of a mono-deuterated methyl group. These results suggest that Chl b is converted into Chla before degradation. Quantification proves that the initial ratio of Chl a:Chl b in the green plant is preserved to about 60–70% in the catabolite composition isolated from yellowing leaves. The incorporation of only one deuterium atom indicates the involvement of two distinguishable redox enzymes during the conversion. Chl 1The abbreviations used are: Chl, chlorophyll; Chlid, chlorophyllide; Pheo, pheophorbide; AcOEt, ethyl acetate; AcMe, acetone; AcOH, acetic acid; CH2Cl2, dichloromethane; EtOH, ethanol; MeOH, methanol; dn, hn, number of attached deuterium or hydrogen atoms in a molecule; ppm, parts per million; MS, mass spectroscopy; amu, atomic mass units.1The abbreviations used are: Chl, chlorophyll; Chlid, chlorophyllide; Pheo, pheophorbide; AcOEt, ethyl acetate; AcMe, acetone; AcOH, acetic acid; CH2Cl2, dichloromethane; EtOH, ethanol; MeOH, methanol; dn, hn, number of attached deuterium or hydrogen atoms in a molecule; ppm, parts per million; MS, mass spectroscopy; amu, atomic mass units. b occurs as an accessory pigment of the light harvesting systems in higher plants, green algae, Euglenaceae and Prochlorophyta and comprises up to 30% of the total Chls (1Scheer H. Scheer H. Chlorophylls. CRC Press, Inc., Boca Raton, FL1991: 3-30Google Scholar). As a matter of fact, although both Chla and b catabolites were found in the green algaChlorella protothecoides, only catabolites originating from Chl a were isolated from higher plants (2Hörtensteiner S. Vincentini F. Matile P. New Phytol. 1995; 129: 237-246Crossref PubMed Scopus (152) Google Scholar, 3Curty C. Engel N. Phytochemistry. 1996; 42: 1531-1536Crossref Scopus (77) Google Scholar). The following observations have led to the hypothesis that in higher plants Chlb is converted into Chl a before degradation: (i) A system comprising isolated etioplasts of cucumber Cucumis sativus showed that chlorophyllide b is converted to Chl a (4Ito H. Tanaka Y. Tsuji H. Tanaka A. Arch. Biochem. Biophys. 1993; 306: 148-151Crossref PubMed Scopus (67) Google Scholar). Subsequent studies of a system consisting of barley (Hordeum vulgare) etioplasts showed that chlorophyllide b is converted via 71-hydroxy Chla to Chl a; both steps required the presence of ATP in the incubation mixture (5Ito H. Ohtsuka T. Tanaka A. J. Biol. Chem. 1996; 271: 1475-1479Abstract Full Text Full Text PDF PubMed Scopus (104) Google Scholar). (ii) In vitro chlorophyll degradation experiments with membrane fractions of senescent chloroplasts of rape cotyledons (Brassica napus) have shown that Pheo b is refused as substrate of the ring cleaving pheophorbide oxygenase under the condition that Pheo a is accepted (2Hörtensteiner S. Vincentini F. Matile P. New Phytol. 1995; 129: 237-246Crossref PubMed Scopus (152) Google Scholar). (iii) Zn(II) Pheo b was converted to Zn(II) 71-hydroxy Chl a in intact barley etioplasts, the reduction required NADPH or NADH. NADH was found to be less effective, ATP was not essential (6Scheumann V. Ito H. Tanaka A. Schoch S. Rüdiger W. Eur. J. Biochem. 1996; 242: 163-170Crossref PubMed Scopus (41) Google Scholar). (iv) Fully senescent cotyledons of rape (B. napus) contain amounts of Chl acatabolites 7a-c accounting for 90% of total Chls originally present in the mature leaf tissue (2Hörtensteiner S. Vincentini F. Matile P. New Phytol. 1995; 129: 237-246Crossref PubMed Scopus (152) Google Scholar, 7Mühlecker W. Kräutler B. Ginsburg S. Matile P. Helv. Chim. Acta. 1993; 76: 2976-2980Crossref Scopus (61) Google Scholar). Chl a to Chl b conversion appears now to be part of a general Chl a(b) interconversion cycle, which is considered to play an important role in the formation and reorganization of the photosynthetic apparatuses (5Ito H. Ohtsuka T. Tanaka A. J. Biol. Chem. 1996; 271: 1475-1479Abstract Full Text Full Text PDF PubMed Scopus (104) Google Scholar) and which enables plants to adapt to high and low light conditions by adjusting the ratio Chl a:Chl b from 3.8–4.8 to 2.7–3.0, respectively (8Porra R.J. Thompson W.A. Kriedmann P.E. Biochim. Biophys. Acta. 1989; 975: 384-394Crossref Scopus (4534) Google Scholar). In vivo labeling experiments with heavy water to elucidate biogenesis mechanisms are barely mentioned in the literature. The method has been applied to study peripheral changes of the porphyrin system during the biosynthesis of bacteriochlorophyll a in the photosynthetic bacterium Rhodospirillum rubrum (9Dougherty R.C. Crespi H.L. Strain H.H. Katz J.J. J. Amer. Chem. Soc. 1966; 88: 2854-2855Crossref Scopus (13) Google Scholar, 10Katz J.J. Dougherty R.C. Crespi H.L. Strain H.H. J. Amer. Chem. Soc. 1966; 88: 2856-2875Crossref Scopus (13) Google Scholar) and to follow the insertion of a deuteron during the light induced cyclization of dark synthesized acyclic carotenoide precursors in the green alga Senedesmus obliquus (11Britton G. Lockley W. Powls R. Goodwin T. Heyes L.M. Nature. 1977; 268: 81-82Crossref Scopus (18) Google Scholar). Recently we have demonstrated by in vivo deuterium labeling experiments withC. protothecoides that in the last step of the macrocyclic ring cleavage a hydrogen atom is highly stereoselectively inserted in the catabolite (12Curty C. Engel N. Plant Physiol. Biochem. 1997; 35: 707-711Google Scholar). In this work we evince by spectroscopic methods that during the de-greening of barley leaves (H. vulgare) in heavy water a fraction of the Chl a catabolite is deuterium labeled; specifically one deuterium atom is incorporated in the methyl group of the apparent chlorophyll a catabolite. The results suggest that Chl b is converted to Chl a by two different cofactors. All chemicals were reagent grade; all solvents were distilled before use. Heavy water containing 80 atom % deuterium was supplied from Armar AG, CH-5312 Döttingen (Switzerland). Thin layer chromatography aluminum foils pre-coated with silica gel 60PF254+366 (0.2 mm) and silica gel 60PF (0.040–0.063 mm) for column chromatography were purchased from Merck, Darmstadt, Germany and 35cc Sep-Pack® Vac C-18, 10 g from Waters (Milford, MA). Barley seeds (H. vulgare L. cv. Gerbel) were a gift from Florimond Desprez, Cappelle-en-Pévèle 59242 Templeuve, France. The seeds were germinated in high density (5 seeds/cm2) in moist garden soil, purchased from a local market, and grown for about 7–10 days in natural light until the primary leaves reached about 10–15 cm in height. 1H-, 13C-, and 2H-NMR measurements were performed on a Bruker Avance DRX-500 spectrometer operating at the frequencies of 500.13, 125.75, or 76.77 MHz, respectively. Samples were dissolved in CDCl3. Chemical shifts were recorded in ppm downfield from tetramethylsilane except for deuterium NMR in which CDCl3, δ = 7.27 ppm was used as internal standard. 1H-Spectra for the labeled material were recorded at a resolution of 7.63·10−5 ppm/data point. Gaussian multiplication of the free induction decay (13Sanders J.K.M. Hunter B.K. Modern NMR Spectroscopy. Oxford University Press, Oxford1990Google Scholar, 14Thiele H. Germanus A. Paape R. Krygsman P. 1D Win-NMR Manual, Release 940701. Brucker-Franzen Analytik GmbH, Bremen, Germany1994Google Scholar) was performed on the NMR-Unix station with UXNMR version 2.1. (Parameters used: Gaussian broadening = 0.5 Hz, line broadening = −0.55 Hz). Mass spectra were obtained with a Bruker FTMS 4.7T BioAPEXII, using chemical ionization (CI) or electrospray ionization techniques in the positive mode. Electrospray ionization spectra were expanded in the range of the molecular ion up to a resolution of 150,000. The most recent IUPAC data for atomic mass and natural abundance of the elements were used to calculate exact molecular masses (15Commission on Atomic Weights and Isotopic Abundances Report for the International Union of Pure and Applied Chemistry Pure Appl. Chem. 1998; 70: 217-235Crossref Scopus (787) Google Scholar) The procedure was similar as described previously (16Kräutler B. Jaun B. Bortlik K. Schellenberg M. Matile P. Angew. Chem. Int. Ed. Engl. 1991; 30: 1315-1318Crossref Scopus (166) Google Scholar) but with the following modifications: To arrest chlorophyll biosynthesis the green intact shoots were left at 25 °C for 12 h in permanent darkness. Afterward, batches of green primary leaves (100 g wet weight; 12 g dry weight) were cut 10–15 cm from the apex and immersed with their ends in heavy water (100 ml, 80 atom % 2H). The opening of the 1,000 ml beakers was covered with punctured aluminum foil to allow gas exchange. The leaves were subsequently incubated at 25 °C during 7–8 days in permanent darkness. When the green color of the Chls had vanished, the yellowish still turgid leaves were collected and stored frozen until use. Unlabeled natural material was obtained accordingly using tap water instead of heavy water. The watering layer was sporadically sampled, and the deuterium content of the water was determined by standard1H-NMR (360 MHz) procedure in which the remaining proton signal in the samples was measured. A sealed capillary filled with acetone was used as external proton standard whose signal area was determined from the area of pure water (H2O) set to 100 atom % 1H; a relaxation delay of 60 s was applied during measurements to the sample. De-greened yellow leaves of H. vulgare (150 g wet weight) were homogenized in a blender with a mixture of 0.1m potassium phosphate buffer, pH 6.8:AcMe:MeOH = 1:1:1 (300 ml). The resultant slurry was filtered over two layers of cotton gauze, the residue was washed with the disintegration buffer (2 × 150 ml). The collected filtrates were centrifuged at 5,000 ×gav for 10 min. Pellets were discarded and the supernatants were extracted with CH2Cl2 (2 × 400 ml). After phase separation the aqueous layer was shortly evaporated in vacuo to remove residual solvent. The remaining solution (200 ml) was filtered through a reversed phase column (35cc Sep-Pack® Vac C-18 cartridges). Afterward the cartridge was washed with 0.1 m potassium phosphate buffer, pH 6.8 (50 ml) and eluted with a 0.1 m potassium phosphate buffer, pH 6.8:AcMe = 1:1 (150 ml) solution. Retention and elution of the catabolite in the cartridge was controlled by a microscale chromic acid degradation assay using aliquots of the eluate (vide infra). Positive reacting fractions were pooled (120 ml), the volatile organic solvent was withdrawn in vacuo leaving a dark brown aqueous phase (60 ml). A solution consisting of 2n H2SO4 and 1% CrO3 (60 ml) was added with stirring at room temperature for 5 min. The resulting solution was continuously extracted overnight with diethyl ether. The sodium sulfate dried ether phase was evaporated to incipient dryness, and the residue was applied to four TLC plates. The plates were developed in CH2Cl2/AcOEt/EtOH/AcOH (50:10:5:0.5). The section of the TLC foil containing maleimide fragment 9 was cut out and eluted with methanol (50 ml). Evaporation of the filtrate in vacuo left a residue, which was two times purified by microcolumn chromatography (∅ = 4 mm, length = 10 cm) using silica gel as stationary and CH2Cl2/acetone (8:2) as mobile phase. Vacuo evaporation of the effluent afforded 1.7 mg of pure maleimide 9. Accordingly, maleimides 8 and 10 were isolated from the CrO3 oxidation mixture, data not shown. Synthetic material was isolated as CrO3 oxidation product of 3-(2-hydroxyethyl)-4-methyl-pyrrole. The pyrrole was synthesized in two steps 2P. Folly and N. Engel, unpublished results. starting from benzyl-3-methyl-4-methoxycarbonylmethyl-5-methoxycarbonyl-2-pyrrolecarboxylate (18Valasinas A. Hurst J. Frydman B. J. Org. Chem. 1998; 63: 1239-1243Crossref Scopus (2) Google Scholar). The melting point of 9 is 104–109 °C.1 H-NMR: 2.01 (t, J = 0.9 Hz, 3H, H3C(41)), 2.67 (tq,J1 = 6.1 Hz, J2 = 0.9 Hz, 2H, H2C(31)), 3.82 (t,J = 6.1 Hz, 2H, H2C(32)), 7.17 (br, 1H, HN(1)). 13 C-NMR: 8.82 (C41), 27.53 (C31), 60.54(C32), 139.20 + 140.49 (C4 + C3), 171.25 + 171.96 (2 × C=O).MS-CI: 156 ([M + H]+, 100%), 138 ([M + H − H2O]+, 58%), 125 ([M + H − CH2OH]+, 6%). IR(KBr): 3,398 (very strong), 1,712 (very strong), 1,360 (strong), 1,086 (strong), 1,041 (strong), 738 (strong). 200-μl samples were agitated with 200 μl of ether Et2O and 200 μl of chromic acid solution (vide supra). The ether solution was spotted on thin layer chromatography and developed in CH2Cl2:AcMe (8:2); RF(9) = 0.27. The maleimide fragments were visualized with Cl2/benzidine (19Rüdiger W. Hoppe-Seyler's Z. Physiol. Chem. 1969; 350 (and literature cited therein): 1291-1300Crossref PubMed Scopus (86) Google Scholar). Fig. 1shows the constitutional formulae of the catabolites isolated so far and reveals that they are all bile-pigment-like linear tetrapyrroles derived from an oxygenolytic cleavage at the C(4)=C(5) bondage of the former Chls. De-greening experiments were performed with green primary leaves of H. vulgare in heavy water (80 atom %2H) or in tap water, respectively. The crude enriched plant extract was directly subjected to the chromic acid degradation procedure basically developed for porphyrins (19Rüdiger W. Hoppe-Seyler's Z. Physiol. Chem. 1969; 350 (and literature cited therein): 1291-1300Crossref PubMed Scopus (86) Google Scholar, 28Rüdiger W. Angew. Chem. Int. Ed. Engl. 1970; 9: 473-480Crossref PubMed Scopus (30) Google Scholar). The particular maleimide fragment 3-(2-hydroxyethyl)-4-methyl-maleimide (9) (Fig. 2), which contains the characteristic β-hydroxyethyl as marker group of the former Chla catabolite of H. vulgare, was isolated and spectroscopically analyzed. 1H- and 13C-NMR and mass spectra of the synthetic and the unlabeled natural material were alike and in accordance with structure 9. All seven carbon-bound protons were assigned by chemical shift reasoning, coupling constants, and integral values (see "Experimental Procedures"). The N-bound hydrogen atom occurred as single broad signal and the O-bound proton was part of the water peak of the solvent.Figure 2Isolated maleimides 8, 9, and 10 obtained after CrO3 oxidation of an extract from de-greened leaves of H. vulgare. Of the three fragments analyzed by 1H-NMR only a fraction of the methyl group of9 was deuterium labeled. The constitution of the Chla catabolite from H. vulgare 5 (16Kräutler B. Jaun B. Bortlik K. Schellenberg M. Matile P. Angew. Chem. Int. Ed. Engl. 1991; 30: 1315-1318Crossref Scopus (166) Google Scholar) is shown in brackets (not isolated).View Large Image Figure ViewerDownload Hi-res image Download (PPT) The maleimide fragment 9 isolated from the labeling experiment of H. vulgare shows a small additional signal group in close proximity to the methyl group C(41) at δ = 2.012 ppm. 3The number of significant figures (4 sf) are not intended to indicate the accuracy of an absolute δ value but serves to calculate chemical shifts differences. After Gaussian multiplication of the free induction decay and amplification this signal group unambiguously displays the resonance pattern of a mono-deuterated methyl group (Fig. 3). The resonance is centered at δ = 1.995 ppm and appears as a characteristic triplet × triplet. In a double resonance experiment in which the methylene group C(31) at δ = 2.67 ppm was irradiated, the triplet of the tri-protio-methyl group collapsed as expected into a singlet and the signal group into a simple triplet with a coupling constant ofJ1H-2H= 2.4 Hz in a ratio of 1:1:1 (Fig. 3). Both, spin multiplicity and signal ratio immediately evince due to the nuclear spin quantum number I = 1 of deuterium that the number of deuterium atoms in the methyl group equals 1. The mono-deuterated methyl group is up-field shifted by Δδ = 0.017 ppm relative to the tri-protio-methyl group. This effect is within the range commonly observed for primary isotopic effects (29Davis D.B. Christofides J.C. Hoffman R.D. R. Soc. Chem. Spec. Publ. 1988; 68: 147-172Google Scholar, 30Allred A.L. Wilk W.D. Chem. Commun. 1969; 1969: 273Crossref Google Scholar). Integration of the signal of the tri-protio-methyl group versus the mono-deutero-methyl group revealed a proton ratio of about 100:4.7. From this figure a ratio of9:9 -d1 of 100:7.1 was calculated. The 2H-NMR spectrum confirmed the presence of one deuterium atom by a triplet (J1H-2H = 2.4 Hz) centered at δ = 2.1 ppm; no other signals were present except the solvent peak (spectrum not shown). Samples were measured in an ion cyclotron resonance spectrometer equipped with an electrospray ionization inlet. Fig. 4 shows the isotopic fine structure at a resolving power of 150,000. The observed molecular peak ion [12C71H914N16O323Na]+was calibrated to m/z 178.048 and an integral value of 100. Table I opposes the calculated and measured values. The signals are base line separated exhibiting the expected mass difference of 3 × 10−3 amu. The ion at 179.051 amu [12C613C1H914N16O323Na]+contains carbon-13 and shows the predicted abundance of 7.7 rel %, which is because of the 13C natural abundance of 7 × 1.10 rel %. The second satellite signal at 179.054 amu [12C71H82H14N16O323Na]+contains 2H and presents the number of molecules in which one protium is replaced by one deuterium. This fraction occurs with an abundance of 6.2 rel % from which 0.1 rel % was subtracted because of the natural abundance of deuterium of 9 × 0.015. The molar ratio of 9:9-d1 is therefore 100:6.1.Table ICalculated and measured mass spectroscopic data of the unlabeled and labeled maleimide 9 in the range of the nominal masses 178 and 179aIsotopic mass and natural abundance of the constituting elements were taken from the literature (15Commission on Atomic Weights and Isotopic Abundances Report for the International Union of Pure and Applied Chemistry Pure Appl. Chem. 1998; 70: 217-235Crossref Scopus (787) Google Scholar). For the sake of correctness 0.55 · 10−3 amu (rest mass of the electron) were subtracted from the uncharged molecular mass ions.bThe scale was adjusted to the theoretical m/zvalue of the exact molecular mass ion.cSignal hidden in the noise.dThe signals of the isotopomers containing carbon-13 or oxygen-17 are unresolved. Open table in a new tab aIsotopic mass and natural abundance of the constituting elements were taken from the literature (15Commission on Atomic Weights and Isotopic Abundances Report for the International Union of Pure and Applied Chemistry Pure Appl. Chem. 1998; 70: 217-235Crossref Scopus (787) Google Scholar). For the sake of correctness 0.55 · 10−3 amu (rest mass of the electron) were subtracted from the uncharged molecular mass ions. bThe scale was adjusted to the theoretical m/zvalue of the exact molecular mass ion. cSignal hidden in the noise. dThe signals of the isotopomers containing carbon-13 or oxygen-17 are unresolved. The ratio of Chl a:Chl b in the leaves during de-greening was followed by high pressure liquid chromatography of a methanol extract (Fig. 5). At the beginning of the incubation experiment this ratio was determined to be 79:21 (100:26). After 8 days in permanent darkness the incubation was terminated. About 10% Chl a and 24% Chl b of the initial content still remained unchanged in the leaves, which means that about 90% Chla and 76% Chl b had vanished. Under the assumption that both Chls are totally converted into catabolites, a ratio Chl a:Chl b of 81:19 (100:23) should be expected. Random labeling of Chl b in a medium of water containing 80 atom % 2H should yield 80% mono-deuterium labeled Chl a and 20% of a "protio-labeled" Chla catabolite in a ratio9:9-d1 of 100:17.6. As a matter of fact, the deuterium content of the heavy water in the beaker slowly diminished during the incubation period from 80 atom %2H to an equilibrium concentration of 55 atom %2H due to the dilution with protic water contained in the leaves (Fig. 6). Under the assumption that the number of deuterium atoms and the initial volume of 100 ml of water remains constant during the experiment the deuterium content of the leaves at each sampling point was calculated from the deuterium concentration of the watering layer and the equilibrium concentration by Eq. 1.xl=(xt=0−xt=s)(xt=0−xequ)·xequEquation 1 where xl = atom % 2H in the leaves at the sampling time; xt=0 = atom %2H in the water layer at zero time (80%);xt=s = atom % 2H in the water layer at sampling time; xequ = atom % 2H in the water layer at equilibrium (55%).Figure 6Exchange rate between the leaves and the heavy water reservoir. Upper curve, time dependent dilution of the heavy water reservoir due to leaking of ordinary water from the leaves. An equilibrium concentration of 55 atom %2H was reached after about 192 h. Lower curve, the deuterium content in the leaves was calculated from the deuterium content of the watering layer and the equilibrium concentration. The vertically hatched area when subtracted from the total area limited by the dotted equilibrium line furnishes the horizontal hatched area, which represents the total amount of water (H2O) in the leaves during the de-greening period.View Large Image Figure ViewerDownload Hi-res image Download (PPT) The area under the calculated curve, which presents the time course of the relative amounts of 55 atom % 2H in the leaves, was subtracted from the total area given by the square of the equilibrium concentration (55 atom % 2H) and the incubation time (192 h). The difference assigns the total of the relative portion of pure water (H2O) in mixture with 55 atom % 2H in the leaves due to the slow exchange rate. This portion (13.6%) together with the protic fraction of the equilibrium mixture (45%) converts Chl b into the nonlabeled apparent Chl ain an amount of 1.4 and 7.7 rel %, respectively; the sum was therefore subtracted from the portion of Chl b and surcharged to Chla. A theoretical ratio of9:9 -d1 of 100:9.5 was calculated from those figures. This result is in close agreement with the spectroscopic measurements of a9:9 -d1 relation of 100:6.1 for MS and 100:7.1 for 1H-NMR and accounts for 64 and 74%, respectively, of the theoretical value. The overall yield was calculated as follows. According to the literature, 115 g H. vulgare leaves afforded 13 mg of the intact catabolite 5 which represents a recovery rate of 10% of the original Chls (16Kräutler B. Jaun B. Bortlik K. Schellenberg M. Matile P. Angew. Chem. Int. Ed. Engl. 1991; 30: 1315-1318Crossref Scopus (166) Google Scholar). Quantitative conversion with CrO3 oxidation to the maleimide fragment9 should therefore yield 3.7 mg per 150 g leaves. In this labeling experiment 1.7 mg of purified 9 was isolated from 150 g leaves, which represents a yield of 46%. This loss is in agreement with the low yields of maleimides generally obtained from CrO3 oxidation of porphyrins (31Bonnet R. Mc Donagh A.F. Chem. Ind. 1969; 1969: 107-108Google Scholar). The ratio unlabeled to labeled 9 reflects both the isotopic composition of the deuterium concentration in the medium and the exchange and hydrogen transfer reaction, which occur during biodegradation. Formally two hydride ions are required to reduce an aldehyde group to a methyl group. Depending on the mechanism, up to two deuterium atoms per methyl group can be incorporated during the catabolic process of Chl b in the presence of heavy water (Fig. 7). We found that only one deuterium atom was incorporated. This fact demonstrates that of the hydrogen isotopes forming the methyl group of the labeled Chl a catabolite one originates from the formyl group of the former Chl b, one arrives by hydride transfer from an as yet unidentified carbon-bond hydrogen source, and another enters the methyl group as proton/deuteron from the surrounding water (Fig. 8). Enzymatic reduction of an aldehyde group to the corresponding alcohol is generally accomplished by nicotinamide-dependent hydride carriers NAD(P)H (32Walsh C. Enzymatic Reaction Mechanisms, Sect. III. W. H. Freeman and Company, San Francisco1979: 311-357Google Scholar,33Clarke A.R. Dafforn T.R. Sinnot M. Comprehensive Biological Catalysis. III. Academic Press, Toronto1997: 1-82Google Scholar). It is a hallmark of these coenzymes not to exchange with the deuterium of the surrounding medium (34Colowick S.P. van Eys J. Park J.H. Florkin M. Stotz E.H. Comprehensive Biochemistry. Elsevier Science Publishers B.V., Amsterdam1966: 1-98Google Scholar). We assume that a hydride ion is mediated by a NAD(P)+/NAD(P)H between a carbon-bond hydrogen such as for example (poly)saccharides, which were acquired during the phototrophic growth phase of the plant in ordinary water and the formyl group. This assumption is supported by ex vivoexperiments in which NAD(P)H was essential to reduce Zn(II) pheophorbide b to the corresponding 71-hydroxy-Chl a (6Scheumann V. Ito H. Tanaka A. Schoch S. Rüdiger W. Eur. J. Biochem. 1996; 242: 163-170Crossref PubMed Scopus (41) Google Scholar). Reductive elimination of a hydroxyl group is generally a more difficult task due to the strong carbon-oxygen bond. This is the reason why enzymatic examples are rarely found in the literature (5Ito H. Ohtsuka T. Tanaka A. J. Biol. Chem. 1996; 271: 1475-1479Abstract Full Text Full Text PDF PubMed Scopus (104) Google Scholar, 35Stubbe J. Adv. Enzymol. Relat. Areas Mol. Biol. 1990; 63: 349-419PubMed Google Scholar). Nevertheless, the unique electronic arrangement of the cyclic 18-π electron porphyrin system facilitates the formation of a resonance-stabilized carbocation 12 (Fig. 8). This elimination process demands an activator capable to transform the hydroxyl group into a better leaving group. In this context it is noteworthy that ATP, which can act as activator was required for the transformation of chlorophyllide b to Chl a in barley etioplasts (5Ito H. Ohtsuka T. Tanaka A. J. Biol. Chem. 1996; 271: 1475-1479Abstract Full Text Full Text PDF PubMed Scopus (104) Google Scholar) but not for the first reduction step to 71-hydroxy Pheo a (7Mühlecker W. Kräutler B. Ginsburg S. Matile P. Helv. Chim. Acta. 1993; 76: 2976-2980Crossref Scopus (61) Google Scholar). Most recently, it has been demonstrated that the final reduction step is achieved when reduced spinach ferredoxin is added to lysed etioplasts (36Scheumann V. Schoch S. Rüdiger W. J. Biol. Chem. 1998; 273: 35102-35108Abstract Full Text Full Text PDF PubMed Scopus (51) Google Scholar). Ferredoxins participate in electron transfer reactions, electrons are typically provided by an electron transfer chain involving NADH and/or flavoproteins (33Clarke A.R. Dafforn T.R. Sinnot M. Comprehensive Biological Catalysis. III. Academic Press, Toronto1997: 1-82Google Scholar). Therefore, we regard cation 12 as terminal electron acceptor, which becomes reduced by two electrons to the corresponding carbanion. Final quenching of the latter with a proton/deuteron from the aqueous medium would account for the observed statistically mono-deuterium labeling of the methyl group. It has been suggested that 12 and/or 14 (Fig. 8) are possible intermediates (37Porra R.J. Photochem. Photobiol. 1997; 65: 492-516Crossref Scopus (112) Google Scholar). However, 1H- and 2H-NMR spectra show no deuterium label in the ethyl group of the maleimide fragment 9; isomerization occurs, if at all, only very slowly. The catabolic sequence Chl b → Chl a → Chla catabolite is more likely to proceed than a subsequent conversion of an assumed Chl b catabolite for the following reasons: (i) Pheo a oxygenase appears to be highly specific, the enzyme uses Pheo a as substrate but refuses Pheob (vide supra). (ii) Independent proofs have shown that the Chl a(b) converting enzymes are present in higher plants (vide supra). (iii) The proposed cation 12 is stabilized by resonance through the extended electronic 18π-system of the Chl macrocycle, whereas the formation of a corresponding cation from 71-hydroxy-Chl bcatabolite would be less favored by resonance. Chromic acid oxidation of the bile-pigment-like chlorophyll catabolite5 of H. vulgare present in the enriched plant extract afforded in addition to 9 the corresponding maleimides 8 and 10 (Fig. 2). 1H- and 2H-NMR spectroscopic investigation showed that of the three maleimides isolated from the plant extract only maleimide 9was partially mono-deuterium labeled at C(41), all others (data not shown) were not. During de novo biosynthesis of the Chls all methyl groups should become evenly mono-deuterated in heavy water because of the consecutive decarboxylation of uroporphyrinogen III to coproporphyrinogen III by uroporphyrinogen III decarboxylase. This result confirms apart from Chla(b) interconversion the general assumption that angiosperms form no Chls in the dark (17Leeper F.J. Scheer H. Chlorophylls. CRC Press, Inc., Boca Raton, FL1991: 407-431Google Scholar). We are indebted to Florimond Despez, Cappelle-en-Pévèle F-59242 Templeuve for providing us withHordeum vulgare L. cv. Gerbel. We thank F. Fehr and F. Nydegger for the spectroscopic measurements.