Trichoderma reesei CE16 acetyl esterase and its role in enzymatic degradation of acetylated hemicellulose

Background

Trichoderma reesei CE16 acetyl esterase (AcE) is a component of the plant cell wall degrading system of the fungus. The enzyme behaves as an exo-acting deacetylase removing acetyl groups from non-reducing end sugar residues.

Methods

In this work we demonstrate this exo-deacetylating activity on natural acetylated xylooligosaccharides using MALDI ToF MS.

Results

The combined action of GH10 xylanase and acetylxylan esterases (AcXEs) leads to formation of neutral and acidic xylooligosaccharides with a few resistant acetyl groups mainly at their non-reducing ends. We show here that these acetyl groups serve as targets for TrCE16 AcE. The most prominent target is the 3-O-acetyl group at the non-reducing terminal Xylp residues of linear neutral xylooligosaccharides or on aldouronic acids carrying MeGlcA at the non-reducing terminus. Deacetylation of the non-reducing end sugar may involve migration of acetyl groups to position 4, which also serves as substrate of the TrCE16 esterase.

Conclusion

Concerted action of CtGH10 xylanase, an AcXE and TrCE16 AcE resulted in close to complete deacetylation of neutral xylooligosaccharides, whereas substitution with MeGlcA prevents removal of acetyl groups from only a small fraction of the aldouronic acids. Experiments with diacetyl derivatives of methyl β-d-xylopyranoside confirmed that the best substrate of TrCE16 AcE is 3-O-acetylated Xylp residue followed by 4-O-acetylated Xylp residue with a free vicinal hydroxyl group.

General significance

This study shows that CE16 acetyl esterases are crucial enzymes to achieve complete deacetylation and, consequently, complete the saccharification of acetylated xylans by xylanases, which is an important task of current biotechnology.     

Distinct roles of carbohydrate esterase family CE16 acetyl esterases and polymer-acting acetyl xylan esterases in xylan deacetylation

Mass spectrometric analysis was used to compare the roles of two acetyl esterases (AE, carbohydrate esterase family CE16) and three acetyl xylan esterases (AXE, families CE1 and CE5) in deacetylation of natural substrates, neutral (linear) and 4-O-methyl glucuronic acid (MeGlcA) substituted xylooligosaccharides (XOS). AEs were similarly restricted in their action and apparently removed in most cases only one acetyl group from the non-reducing end of XOS, acting as exo-deacetylases. In contrast, AXEs completely deacetylated longer neutral XOS but had difficulties with the shorter ones. Complete deacetylation of neutral XOS was obtained after the combined action of AEs and AXEs. MeGlcA substituents partially restricted the action of both types of esterases and the remaining acidic XOS were mainly substituted with one MeGlcA and one acetyl group, supposedly on the same xylopyranosyl residue. These resisting structures were degraded to great extent only after inclusion of α-glucuronidase, which acted with the esterases in a synergistic manner. When used together with xylan backbone degrading endoxylanase and β-xylosidase, both AE and AXE enhanced the hydrolysis of complex XOS equally.     

Mode of action of acetylxylan esterases on acetyl glucuronoxylan and acetylated oligosaccharides generated by a GH10 endoxylanase

Background

Substitutions on the xylan main chain are widely accepted to limit plant cell wall degradability and acetylations are considered as one of the most important obstacles. Hence, understanding the modes of action of a range of acetylxylan esterases (AcXEs) is of ample importance not only to increase the understanding of the enzymology of plant decay/bioremediation but also to enable efficient bioconversion of plant biomass.

Methods

In this study, the modes of action of acetylxylan esterases (AcXEs) belonging to carbohydrate esterase (CE) families 1, 4, 5 and 6 on xylooligosaccharides generated from hardwood acetyl glucuronoxylan were compared using MALDI ToF MS. Supporting data were obtained by following enzymatic deacetylation by ¹H NMR spectroscopy.

Conclusions

None of the used enzymes were capable of complete deacetylation, except from linear xylooligosaccharides which were completely deacetylated by some of the esterases in the presence of endoxylanase. A clear difference was observed between the performance of the serine-type esterases of CE families 1, 5 and 6, and the aspartate-metalloesterases of family CE4. The difference is mainly due to the inability of CE4 AcXEs to catalyze deacetylation of 2,3-di-O-acetylated xylopyranosyl residues. Complete deacetylation of a hardwood acetyl glucuronoxylan requires additional deacetylating enzyme(s).

General significance

The results contribute to the understanding of microbial degradation of plant biomass and outline the way to achieve complete saccharification of plant hemicelluloses which did not undergo alkaline pretreatment.     

Carbohydrate esterases of family 2 are 6-O-deacetylases

Three acetyl esterases (AcEs) from the saprophytic bacteria Cellvibrio japonicus and Clostridium thermocellum, members of the carbohydrate esterase (CE) family 2, were tested for their activity against a series of model substrates including partially acetylated gluco-, manno- and xylopyranosides. All three enzymes showed a strong preference for deacetylation of the 6-position in aldohexoses. This regioselectivity is different from that of typical acetylxylan esterases (AcXEs). In aqueous medium saturated with vinyl acetate, the CE-2 enzymes catalyzed transacetylation to the same position, i.e., to the primary hydroxyl group of mono- and disaccharides. Xylose and xylooligosaccharides did not serve as acetyl group acceptors, therefore the CE-2 enzymes appear to be 6-O-deacetylases.     

Positional specifity of acetylxylan esterases on natural polysaccharide: An NMR study

Background

Microbial degradation of acetylated plant hemicelluloses involves besides enzymes cleaving the glycosidic linkages also deacetylating enzymes. A detailed knowledge of the mode of action of these enzymes is important in view of the development of efficient bioconversion of plant materials that did not undergo alkaline pretreatment leading to hydrolysis of ester linkages.

Methods

In this work deacetylation of hardwood acetylglucuronoxylan by acetylxylan esterases from Streptomyces lividans (carbohydrate esterase family 4) and Orpinomyces sp. (carbohydrate esterase family 6) was monitored by ¹H-NMR spectroscopy.

Results

The ¹H-NMR resonances of all acetyl groups in the polysaccharide were fully assigned. The targets of both enzymes are 2- and 3-monoacetylated xylopyranosyl residues and, in the case of the Orpinomyces sp. enzyme, also the 2,3-di-O-acetylated xylopyranosyl residues. Both enzymes do not recognize as a substrate the 3-O-acetyl group on xylopyranosyl residues α-1,2-substituted with 4-O-methyl-d-glucuronic acid.

Conclusions

The ¹H-NMR spectroscopy approach to study positional and substrate specificity of AcXEs outlined in this work appears to be a simple way to characterize catalytic properties of enzymes belonging to various CE families.

Significance

The results contribute to development of efficient and environmentally friendly procedures for enzymatic degradation of plant biomass.     

Preparation of regioselectively feruloylated p-nitrophenyl α-l-arabinofuranosides and β-d-xylopyranosides—convenient substrates for study of feruloyl esterase specificity

p-Nitrophenyl α-l-arabinofuranoside and β-d-xylopyranoside mono-O-ferulates were prepared by 4-O-acetylferuloylation of corresponding enzymatically prepared di-O-acetates followed by deacetylation. An alternative mild acylation catalysed by zinc oxide was tested on xylopyranoside derivatives. The chemoselective methanolysis of the acetyl groups using neutral catalyst dibutyltin oxide at reflux was used as deacetylation method. Under these conditions a significant feruloyl migration was observed mainly on p-nitrophenyl 3-O-feruloyl-β-d-xylopyranoside resulting in low yields of the positional isomers. Investigation of substrate and positional specificity of different types of feruloyl esterases on the presented compounds in enzyme-coupled assays was reported previously.     

Microbial carbohydrate esterases deacetylating plant polysaccharides

Several plant polysaccharides are partially esterified with acetic acid. One of the roles of this modification is protection of plant cell walls against invading microorganisms. Acetylation of glycosyl residues of polysaccharides prevents hydrolysis of their glycosidic linkages by the corresponding glycoside hydrolases. In this way the acetylation also represents an obstacle of enzymatic saccharification of plant hemicelluloses to fermentable sugars which appears to be a hot topic of current research. We can eliminate this obstacle by alkaline extraction or pretreatment leading to saponification of ester linkages. However, this task has been accomplished in a different way in the nature. The acetyl groups became targets of microbial carbohydrate esterases that evolved to overcome the complexity of the plant cell walls and that cooperate with glycoside hydrolases in plant polysaccharide degradation. This article concentrates on enzymes deacetylating plant hemicelluloses excluding pectin. They are currently grouped in at least 8 families, specifically in CE families 1–7 and 16, originally assigned as acetylxylan esterases, the enzymes acting on hardwood acetyl glucuronoxylan and its fragments generated by endo-β-1,4-xylanases. There are esterases deacetylating softwood galactoglucomannan, but they have not been classified yet. The enzymes present in CE families 1–7 differ in structure and substrate and positional specificity. There are families behaving as endo-type and exo-type deacetylates, i.e. esterases deacetylating internal sugar residues of partially acetylated polysaccharides and also esterases deacetylating non-reducing end sugar residues in oligosaccharides. With one exception, the enzymes of all mentioned CE families belong to serine type esterases. CE family 4 harbors enzymes that are metal-dependent aspartic esterases. Three-dimensional structures have been solved for members of the first seven CE families, however, there is still insufficient knowledge about their substrate specificity and real physiological role. Current knowledge on catalytic properties of the selected families of CEs is summarized in this review. Some of the families are emerging also as new biocatalysts for regioselective acylation and deacylation of carbohydrates.     

Synthesis of Quinoxaline Azido and Amino Reverse Ribofuranoside and Their O-Regioisomers

A series of quinoxaline azido reverse nucleosides 3a-c and their O-regioisomers 4a-c was prepared by reaction of quinoxaline 1a-c with 3-azido-3-deoxy-1,2-O-isopropylidene-5-p-toluenesulfonyl-D-ribofuranose (2) in the presence of sodium hydride. Structure modification of these interesting structures includes reduction and the subsequent acetylation reactions to give quinoxaline amino and acetyl amino reverse nucleosides and their O-regioisomers.     

Action of acetylxylan esterase from Trichoderma reesei on acetylated methyl glycosides

Substrate specificity of purified acetylxylan esterase (AcXE) from Trichoderma reesei was investigated on partially and fully acetylated methyl glycopyranosides. Methyl 2,3,4-tri-O-acetyl-β-

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-xylopyranoside was deacetylated at positions 2 and 3, yielding methyl 4-O-acetyl-β-

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-xylopyranoside in almost 90% yield. Methyl 2,3-di-O-acetyl β-

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-xylopyranoside was deacetylated at a rate similar to the fully acetylated derivative. The other two diacetates (2,4- and 3,4-), which have a free hydroxyl group at either position 3 or 2, were deacetylated one order of magnitude more rapidly. Thus the second acetyl group is rapidly released from position 3 or 2 after the first acetyl group is removed from position 2 or 3. The results strongly imply that in degradation of partially acetylated β-1,4-linked xylans, the enzyme deacetylates monoacetylated xylopyranosyl residues more readily than di-O-acetylated residues. The T. reesei AcXE attacked acetylated methyl β-

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-glucopyranosides and β-

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-mannopyranosides in a manner similar to the xylopyranosides.     

CVI. Total synthesis of the structural gene for an alanine transfer ribonucleic acid from yeast. Synthesis of two nonanucleotides and a heptanucleotide corresponding to nucleotide sequences 22 to 30, 41 to 49 and 28 to 34

Two nonadeoxynucleotides with the sequences, d-C-T-A-A-G-G-G-A-G (nonanucleotide-I) and d-T-C-T-C-C-G-G-T-T (nonanucleotide-II), and a heptadeoxynucleotide having the sequence, d-A-G-A-G-T-C-T, have been chemically synthesized. These polynucleotides represent, respectively, the nucleotide sequences 22 to 30, 41 to 49, and 28 to 34 of the gene for yeast alanine transfer RNA (Fig. 1). The synthetic steps used in the synthesis of the nonanucleotide-I were: the condensation of the protected nucleoside, d-MMTr-C^An, with the protected nucleotide, d-pT-OAc, to give the dinucleotide, d-MMTr-C^AnpT; the condensation of the dinucleotide with d-pA^Bz-OAc to give the trinucleotide, d-MMTr-C^AnpTpA^Bz; the condensation of the latter with the dinucleotide, d-pA^BzpG^1B-OAc, to give the pentanucleotide, d-MMTr-C^AnpTpA^BzpA^BzpG^1B; the condensation of this pentanucleotide with d-pG^1BpG^1B-OAc to give the protected heptanucleotide, d-MMTr-C^AnpTpA^BzpA^BzpG^1BpG^1BpG^1B, and finally, the condensation of this heptanucleotide with the dinucleotide, d-pA^BzpG^1B-OAc, to give the protected nonanucleotide, d-MMTr-C^AnpTpA^BzpA^BzpG^1BpG^1BpG^1BpA^BzpG^1B. The steps used in the synthesis of the nonanucleotide-II were: the condensation of d-MMTr-T with the tetranucleotide, d-pC^AnpTpC^AnpC^An-OAc, to give the pentanucleotide, d-MMTr-TpC^AnpTpC^AnpC^An; the condensation of the latter with the dinucleotide, d-pG^1BpG^1B-OAc, to give the heptanucleotide, d-MMTr-TpC^An-pTpC^AnpC^AnpG^1BpG^1B, and finally, the condensation of the heptanucleotide with the dinucleotide, d-pTpT-OAc, to give the protected deoxynonanucleotide, d-MMTr-TpC^AnpTpC^AnpC^AnpG^1BpG^1BpTpT. For the synthesis of the heptanucleotide, A-G-A-G-T-C-T, the 5′-monocyanoethyl tetranucleotide, d-CEpA^Bz-pG^1BpA^BzpG^1B, was condensed with the trinucleotide, d-pTpC^AnpT-OAc, to give the protected heptanucleotide, d-pA^BzpG^1BpA^BzpG^1BpTpC^AnpT. After removal of the N-protecting groups, the completely deprotected nonanucleotides, as well as the intermediate oligonucleotides and the heptanucleotide, d-A-G-A-G-T-C-T, were purified further by a combination of paper and column chromatography.     

Covalent anthocyanin–flavonol complexes from the violet-blue flowers of Allium ‘Blue Perfume’

Three covalent anthocyanin–flavonol complexes (pigments 1–3) were extracted from the violet-blue flower of Allium ‘Blue Perfume’ with 5% acetic acid-MeOH solution, in which pigment 1 was the dominant pigment. These three pigments are based on delphinidin 3-glucoside as their deacylanthocyanin and were acylated with malonyl kaempferol 3-sophoroside-7-glucosiduronic acid or malonyl-kaempferol 3-p-coumaroyl-tetraglycoside-7-glucosiduronic acid in addition to acylation with acetic acid.By spectroscopic and chemical methods, the structures of these three pigments 1–3 were determined to be: pigment 1, (6^I-O-(delphinidin 3-O-(3^I-O-(acetyl)-β-glucopyranoside^I)))(2^VI-O-(kaempferol 3-O-(2^II-O-(3^III-O-(β-glucopyranosyl^V)-β-glucopyranosyl^III)-4^II-O-(trans-p-coumaroyl)-6^II-O-(β-glucopyranosyl^IV)-β-glucopyranoside^II)-7-O-(β-glucosiduronic acid^VI))) malonate; pigment 2, (6^I-O-(delphinidin 3-O-(3^I-O-(acetyl)-β-glucopyranoside^I)))(2^VI-O-(kaempferol 3-O-(2^II-O-β-glucopyranosyl^III)-β-glucopyranoside^II)-7-O-(β-glucosiduronic acid^VI))); and pigment 3, (6^I-O-(delphinidin 3-O-(3^I-O-(acetyl)-β-glucopyranoside^I)))(2^VI-O-(kaempferol 3-O-(2^II-O-(3^III-O-(β-glucopyranosyl^V)-β-glucopyranosyl^III)-4^II-O-(cis-p-coumaroyl)-6^II-O-(β-glucopyranosyl^IV)-β-glucopyranoside^II)-7-O-(β-glucosiduronic acid^VI))) malonate.The structure of pigment 2 was analogous to that of a covalent anthocyanin–flavonol complex isolated from Allium schoenoprasum where delphinidin was observed in place of cyanidin. The three covalent anthocyanin–flavonol complexes (pigment 1–3) had a stable violet-blue color with three characteristic absorption maxima at 540, 547 and 618 nm in pH 5–6 buffer solution. From circular dichroism measurement of pigment 1 in the pH 6.0 buffer solution, cotton effects were observed at 533 (+), 604 (−) and 638 (−) nm. Based on these results, these covalent anthocyanin–flavonol complexes were presumed to maintain a stable intramolecular association between delphinidin and kaempferol units closely related to that observed between anthocyanin and hydroxycinnamic acid residues in polyacylated anthocyanins. Additionally, an acylated kaempferol glycoside (pigment 4) was isolated from the same flower extract, and its structure was determined to be kaempferol 3-O-sophoroside-7-O-(3-O-(malonyl)-β-glucopyranosiduronic acid).     

CVII. Total synthesis of the structural gene for an alanine transfer ribonucleic acid from yeast. Synthesis of a dodecadeoxynucleotide and a hexadeoxynucleotide corresponding to the nucleotide sequence 1 to 12

A dodecadeoxynucleotide having the sequence, d-T-G-G-T-G-G-A-C-G-A-G-T, and a hexanucleotide having the sequence, d-C-C-A-C-C-A, have been chemically synthesized. These compounds represent, respectively, the nucleotide sequence 1 to 12 of one strand and 1 to 6 of the complementary strand of the gene corresponding to yeast alanine transfer RNA. The synthesis of the dodecanucleotide started with the condensation of 5′-O-monomethoxytrityl thymidine (d-MMTr-T) with N-benzoyl-3′-O-acetyl deoxyguanosine 5′-phosphate (d-pg^BZ-OAc) to give the dinucleotide, d-MMTr-TpG^BZ. Successive condensations of suitability protected mononuoleotides with the 3′-hydroxyl end of the growing chain gave the protected heptanucleotide, d-MMTr-TpG^BZpG^BZpTpG^BZpG^BZpA^BZ. The protected heptanucleotide was then condensed with the dinucleotide, d-pC^ANpG^BZ-OAc, to give the nonanucleotide, d-MMTr-TpG^BZpG^BZpTpG^BZpG^BZpA^BZpC^ANpG^BZ. Condensation of the nonanucleotide with the protected trinucleotide, d-pA^BZpG^BZpT-OAc, gave the protected dodecanucleotide, d-MMTr-TpG^BZpG^BZpTpG^BZpG^BZ-pA^BZpC^ANpGr^BZpA^BZpG^BZpT. The condensing agents used were dicyclohexylcarbodiimide, tri-isopropylbenzenesulfonyl chloride and mesitylenesulfonyl chloride. After removal of the protecting groups, the completely deprotected dodecanucleotide was further purified by anion-exchange chromatography in the presence of 7 M-urea. The steps involved in the synthesis of the hexanucleotide were: the condensation, of 5′-O-cyanoethyl phosphate of N₍₄₎-anisoyl deoxycytidylyl-(3′ → 5′)MN₍₄₎aniaoyl deoxycytidine, d-CEpC^AnpC^An, with d-pA^BZ-OAc to give the protected trinucleotide, d-pC^AnpC^AnpA^BZ, and the condensation of cyanoethyl derivative of the trinucleotide (d-CEpC^AnpC^AnpA^BZ) with the trinucleotide, d-pC^AnpC^AnpA^BZ-OAc, to give the protected hexanucleotide, d-pC^AnpC^AnpA^BZpC^AnpC^AnpA^BZ. After removal of the N-protecting groups the 5′-phosphate group was removed by treatment with bacterial alkaline phosphatase and the hexanucleotide, d-C-C-A-C-C-A, was isolated by paper chromatography. The yields varied between 20 and 80% at different steps.     

Anthocyanins from red flowers of Camellia cultivar 'Dalicha'

Five anthocyanins, cyanidin 3-O-(2-O-β-xylopyranosyl-6-O-(Z)-p-coumaroyl)-β-galactopyranoside (2), cyanidin 3-O-(2-O-β-xylopyranosyl-6-O-(E)-p-coumaroyl)-β-galactopyranoside (3), cyanidin 3-O-(2-O-β-xylopyranosyl-6-O-(E)-caffeoyl)-β-galactopyranoside (4), cyanidin 3-O-(2-O-β-xylopyranosyl-6-O-acetyl)-β-galactopyranoside (5), and cyanidin 3-O-(2-O-β-xylopyranosyl-6-O-acetyl)-β-glucopyranoside (6), together with the known cyanidin 3-O-(2-O-β-xylopyranosyl)-β-galactopyranoside (1), were isolated from red flowers of Camellia cultivar ‘Dalicha’ (Camellia reticulata) by chromatography using open columns. Their structures were subsequently determined on the basis of spectroscopic analyses, i.e., ¹H NMR, ¹³C NMR, HMQC, HMBC, HR ESI-MS and UV-vis.     

Mutations of Arabidopsis TBL32 and TBL33 Affect Xylan Acetylation and Secondary Wall Deposition

Xylan is a major acetylated polymer in plant lignocellulosic biomass and it can be mono- and di-acetylated at O-2 and O-3 as well as mono-acetylated at O-3 of xylosyl residues that is substituted with glucuronic acid (GlcA) at O-2. Based on the finding that ESK1, an Arabidopsis thaliana DUF231 protein, specifically mediates xylan 2-O- and 3-O-monoacetylation, we previously proposed that different acetyltransferase activities are required for regiospecific acetyl substitutions of xylan. Here, we demonstrate the functional roles of TBL32 and TBL33, two ESK1 close homologs, in acetyl substitutions of xylan. Simultaneous mutations of TBL32 and TBL33 resulted in a significant reduction in xylan acetyl content and endoxylanase digestion of the mutant xylan released GlcA-substituted xylooligomers without acetyl groups. Structural analysis of xylan revealed that the tbl32 tbl33 mutant had a nearly complete loss of 3-O-acetylated, 2-O-GlcA-substituted xylosyl residues. A reduction in 3-O-monoacetylated and 2,3-di-O-acetylated xylosyl residues was also observed. Simultaneous mutations of TBL32, TBL33 and ESK1 resulted in a severe reduction in xylan acetyl level down to 15% of that of the wild type, and concomitantly, severely collapsed vessels and stunted plant growth. In particular, the S2 layer of secondary walls in xylem vessels of tbl33 esk1 and tbl32 tbl33 esk1 exhibited an altered structure, indicating abnormal assembly of secondary wall polymers. These results demonstrate that TBL32 and TBL33 play an important role in xylan acetylation and normal deposition of secondary walls.     

Configurational assignments of C-nitromethyl-C-hydroxy branched-chain carbohydrate derivatives by use of a europium shift-reagent in 1 H-N.M.R. spectroscopy

Configurational assignments for the tertiary alcoholic centers of four branched-chain 3-C-nitromethylglycopyranosides, namely, methyl 2-benzamido-4,6-O-benzylidene-2-deoxy-3-C-nitromethyl-α-D-allopyranoside (1), benzyl 2-acetamido-4,6-O-benzylidene-2-deoxy-3-C-nitromethyl-α-D-glucopyranoside (4), benzyl 2-acetamido-4,6-O-benzylidene-2-deoxy-3-C-nitromethyl-α-D-allopyranoside (5), and methyl 4,6-O-benzylidene-3-C-nitromethyl-2-O-p-tolylsulfonyl-α-D-glucopyranoside (8), were made on the basis of the downfield chemical shifts of their identifiable protons per molar equivalent of added Eu(fod)₃, as compared with those of model compounds, of known configuration, having a close structural relationship. In some cases, the assignments were corroborated by the position of the acetyl resonances in the unshifted 60-MHz p.m.r. spectra of the corresponding O-acetyl derivatives.     

Chromone acyl glucosides and an ayanin glucoside from Dasiphora parvifolia

Two new chromone acyl glucosides, 5-hydroxy-7-O-(6-O-p-cis-coumaroyl-β-D-glucopyranosyl)-chromone (1) and 5-hydroxy-7-O-(6-O-p-trans-coumaroyl-β-D-glucopyranosyl)-chromone (2), and a new flavonoid glucoside, ayanin 3′-O-β-D-glucopyranoside (3) were isolated from aerial parts of Dasiphora parvifolia, together with flavonoid glycosides (4–10), catechins (11, 12), and hydrolysable tannins (13, 14). The chemical structures of these compounds were elucidated on the basis of spectroscopic data. The 1,1-diphenyl-2-picrylhydrazyl (DPPH) radical scavenging activity and the hyaluronidase inhibitory activity of these compounds were evaluated.     

Isolation from a softwood xylan of oligosaccharides containing two 4-O-methyl-d-glucuronic acid residues

Partial hydrolysis of a larch arabino(4-O-methylglucurono)xylan afforded two series of oligouronides composed of 4-O-methyl- d-glucuronic acid and d-xylose residues. The first series included aldouronic acids up to the aldopentaouronic acid. Methylation analysis indicated that the aldopentao- and aldotetrao-uronic acids were mixtures of isomers. One aldotetraouronic acid was isolated and identified as O-β-d-Xylp-(1 → 4)-O-β-d-Xylp-(1 → 4)-O-(4-O-Me-α-d-GlcAp)-(1 → 2)-d-Xyl. The two isomeric aldotriouronic acids were separated from each other. The acids of the second series, which were composed of two uronic acids and 2-4 d-xylose residues, were identified as follows: O-β-d-Xylp-(1 → 4)-O-(4-O-Me-α-d-GlcAp)-(1 → 2)-O-β-d-Xylp-(1 → 4)-O(4-O-Me-α-d-GlcAp)-(1 → 2)-O-β-d-Xylp-(1 → 4)-d-Xyl, O-(4-O-Me-α-d-GlcAp)-(1 → 2)-O-β-d-Xylp-(1 → 4)-O-(4-O-Me-α-d-GlcAp)-(1 → 2)-O-β-d-Xylp-(1 → 4)-O-β-d -Xylp-(1 → 4)-D-Xyl, O-(4-O-Me-α-d-GlcAp)-(1 → 2)-O-β-d-Xylp-(1 → 4)-O-(4-O-Mec-α-d-GlcAp)-(1 → 2)-O-β-d-Xylp-(1 → 4)-D-Xyl, and O-(4-O-Me-α-d-GlcAp)-(1 → 2)-O-β-d-Xylp-(1 → 4)-O-(4-O-Me-α-d-GlcAp)-(1 → 2)-D-Xyl. The first three compounds were new acidic oligosaccharides. The 4-O-methyl-d-glucuronic acid in the second series was present in a larger proportion than in the first series, indicating that a large proportion of the uronic acid side-chains were located on two contiguous D-xylose residues in the backbone of the softwood xylan.     

N-[1-13C]acetylimidazole as a reagent for tyrosyl modification in protein NMR studies: acetylation of cytochrome c

The reaction of N-[1-¹³C] acetylimidazole with cytochrome c and guanidinated cytochrome c was evaluated as a means of introducing NMR-detectable groups as conformation-dependent probes. Resonances from both N-[1-¹³C]acetyl lysyl and O-[1-¹³C]acetyl tyrosyl groups were observed when ferricytochrome c was acetylated. However, only O-[1-¹³C]acetyl tyrosyl resonances were seen with acetylated guanidinated ferricytochrome c. Chemical shifts of the four O-[1-¹³C]acetyl tyrosyl groups were conformation dependent and ranged from 172 to 176 ppm. A convenient method for the preparation of N-[1-¹³C]acetylimidazole is described.     

The chemical synthesis of glucosaminylphosphatidylglycerol. Comparison with a new phospholipid isolated from Bacillus megaterium

1. We describe the synthesis of a glucosamine derivative of phosphatidylglycerol having the same structure as that of the natural compound isolated from Bacillus megaterium. 2. 2-O-(3,4,6-Tri-O-acetyl-2-deoxy-2-phthalimido-d-glucopyranosyl)-3-O-benzyl-1-iodo-sn-glycerol was prepared by a Königs–Knorr condensation between 3-O-benzyl-1-toluene-p-sulphonyl-sn-glycerol and 3,4,6-tri-O-acetyl-1-bromo-2-deoxy-2-phthalimido-d-glucopyranose followed by replacement of the toluene-p-sulphonyl group with iodine. The iodide was treated with the silver salt of 2-isolauroyl-1-oleoyl-sn-glycerol 3-(monobenzyl hydrogen phosphate) to form the fully protected phosphoglycolipid. 3. Removal of benzyl protecting groups by catalytic hydrogenolysis, phthaloyl group with hydrazine and acetyl groups with pH10 buffer furnished 2-O-(2-amino-2-deoxy-d-glucopyranosyl)-1-(2-isolauroyl-1-stearoyl-sn-glycero-3-phosphoryl)-sn-glycerol. 4. The synthetic and natural compounds appeared identical when compared by chromatography and by identification of hydrolysis products from chemical and enzymic degradations.     

Substrate Specificity,Mode of Action,and of Inhibition by Organic Acids of Purified Acetylesterase from Sclerotinia Fungus

Acetylesterase (AcE) of Sclerotinia libertiana was purified approximately 1170-fold, and proved homogeneous by electrophoresis, ultracentrifugation and chromatography. The purified AcE hydrolyzed various acetyl esters in the following order; vinyl acetate, tri-acetin, n-butyl acetate, p-nitrophenylacetate, diacetin, ethylene glycol diacetate, monoacetin, ethyl acetate, acetylcholine, methyl acetate. It also had apparently a slight activity on tannic acid, benzoylcholine, methyl butyrate and acetic anhydride.

The mode of AcE reaction on these substrates could be divided into two types of group by Lineweaver-Burk plot, one forms the enzyme-substrate complex, ES, and the other, SES additionally combining substrate at a high substrate concentration.

From the inhibition experiment by organic acids, it was suggested that the neighbouring carboxyl groups of the di-, or tribasic acid such as citric, cis-aconitic, succinic, and maleic acid have a significance on inhibition of the AcE. Also, choline esterase inhibitor partially inhibited the activity on acetylcholine, and bivalent metal ion increased the activity on triacetin. Thus, the AcE was supposed to have a many adjacent sites of interaction with the substrate.