Glycobiology vol. 7 no. 4 pp. 565-570, 1997 Structural and biological roles of glycosylations in pulmonary angiotensin I-converting enzyme Bruno Baudin1'2'3, Nathalie Alves1, Antoine Pilon1, B£n6dicte Be'ne'teau-Burnat1'2 and Jacqueline Giboudeau1 'Laboratoire de Biochimie A, HOpital Saint-Antoine, 184, Rue du Fbg Saint-Antoine, 75571 Paris Cede* 12, France and 2Laboratoire de Biochimie Generale et de Glycobiologie, UFR Pharmacie, University Rent Descartes (Paris V), 4 Avenue de l'Observatoire, 75006 Paris, France 'To whom correspondence should be addressed at: Laboratoire de Biochimie A, H6pital Saint-Antoine, 184, Rue du Fbg Saint-Antoine, 75571 Paris Cedex 12, France We enzymatically deglycosylated pig lung angiotensin I-converting enzyme (ACE) to study the involvement of its glycanic chains in its physicochemical and catalytic properties. The effects of endoglycosidases F 2 and H, and of N-glycanase were assessed by ACE mobility in SDS-PAGE. N-Glycanase only was completely effective with or without previous denaturation, leading to a shift in ACE M r from 172 to 135 kDa; endoglycosidase F 2 produced the same shift but only without previous denaturation. Deglycosylated ACE had the same kcat as native ACE for the substrate hippuryl-histidyl-Ieucine, and an identical Stokes radius as measured by size-exclusion high performance liquid chromatography. Neuraminidase had no effect on ACE Stokes radius but slightly decreased its kcat which could be related to variations in ionization of the active site. The isoelectric point of ACE, as, determined by isoelectric focusing, increased from 4.5-4.8 to 5.0-53 after either endoglycosidase F3 or neuraminidase digestion, but still with microheterogeneities which thus did not seem to be related to ACE glycans. Deglycosylated ACE did not bind onto agaroselectins in contrast to native ACE which bound strongly to concanavalin A showing interactions involving oligomannosidic or biantennary and sialylated N-acetyl-lactosaminic isoglycans. Finally, tunicamycin, an inhibitor of Nglycosylation, did not modify ACE secretion by endothelial cells. Thus, ACE glycans have no drastic effects on structural and biological properties of the protein, but they may have a functional role on intracellular targeting of both secreted and membrane-bound ACE isoforms, also for the protection of the soluble plasma form against hepatic lectins and the maintenance of its hydrosolubility. Key words: angiotensin I—converting enzyme (peptidyldipeptidase EC.3.4.15.1 )/endothelium/glycosidases/lectins Introduction Angiotensin I-converting enzyme (ACE) (or peptidyldipeptide hydrolase EC.3.4.15.1) is a key enzyme in renin-angiotensin and kallikrein-kinin systems, by removing the carboxyterminal dipeptides of angiotensin I and of bradykinin, thereby activating the former into angiotensin II, a vasopressor, and © Oxford University Press degrading the latter, a vasodilator. ACE is a zinc-containing glycoprotein which is expressed in various tissues under different molecular forms, but always with one polypeptide chain. The somatic isoenzyme exhibits two molecular forms, a membrane-bound form and a soluble form. The membrane-bound form is mainly located in vascular endothelial cells as an ectoenzyme (Ryan et al., 1975; Baudin et al, 1996), but also on the brush-border of renal tubular and intestinal epithelial cells (Bruneval et al., 1986) and in monocytes and macrophages (Friedland et al, 1978). Testicular cells synthesize a germinative isoenzyme with a lower molecular mass, around 100 kDa versus around 160 kDa for the somatic enzyme (Iwata et al., 1982; Soubrier et al, 1988). The larger somatic isoenzyme has two highly homologous domains, each bearing a catalytic site, whereas the smaller isoenzyme from germinal cells has a single domain and therefore only one active site and would represent the ancestral, nonduplicated form of the ACE gene (Lattion et al., 1989). A circulating soluble form of ACE is found in blood plasma and is most likely released by the vascular endothelial cells (Das et al., 1977; Beldent et al, 1993). We have previously purified ACE from pig and human lung and blood (Baudin et al, 1991), compared the physicochemical properties and the chemical compositions of both the pulmonary and serum forms (B.Baudin, personal communication), and demonstrated the elongated shape of the pig pulmonary enzyme in aqueous solution (Baudin et al, 1988). In particular, lung ACE appeared to be a glycoprotein containing about 10% (w/w) of sugars, and only those which are characteristic of asparagine N-glycosylation. The aim of the present study was to investigate the involvement of glycosylation in the physicochemical, catalytic, and biosynthetic properties of the enzyme. We carried out comparative analyses before and after digestion with glycosidases. Results and discussion Effect of deglycosylation on ACE Mr and size ACE was purified from pig lung to electrophoretic homogeneity as shown in Figure 1; typically, 2 mg was isolated from 300 g of pulmonary tissue. Several protocols for enzymatic deglycosylation of ACE were compared; N-glycosidases were chosen because pulmonary ACE contains N-asparagine bound glycans only (Hartley and Soffer, 1978; Baudin et al., 1988). Endoglycosidase H was not effective for ACE deglycosylation under the conditions used (not shown). It was not possible to decrease the pH below 5 because ACE precipitated around its isoelectric point (B.Baudin, personal communication). In contrast, both endoglycosidase F 2 , at pH 5.6, and N-glycanase, at pH 8.0, were effective, decreasing ACE mobility in SDSPAGE from 172 ± 4 kDa to 135 ± 4 kDa. Curiously, previous denaturation in SDS did not allow the deglycosylation by endoglycosidase F 2 whereas N-glycanase was effective with or 565 B.Baudin et al Mr X103 ACE -* 45 8 Fig. 1. SDS-PAGE of pig lung ACE before (2, 4) and after digestion with either neuraminidase (1), N-glycanase (5), endoglycosidase F 2 (6), or endoglycosidase H (7), without previous SDS denaturation. High molecular weight standards (3, 8). without previous denaturation of ACE (Figure 1). The lower Mj of deglycosylated ACE is near to that deduced from endothelial cDNA which does not take account of glycan mass (Soubrier et al, 1988). Neuraminidase treatment had no effect on the molecular mass of ACE (Figure 1). It is known that endoglycosidase H hydrolyses more particularly oligomannosidic glycans, that the endoglycosidases F have a greater specificity for N-acetyl-lactosaminic glycans, and that N-glycanase is not specific for a particular type of glycans; thus, our data with these glycosidases show that the glycans of pulmonary ACE are not of one or the other type but rather a mixture of both types or hybrid structures. Previous data with the establishment of sugar molar ratio already predicted a mixture of complex and lactosaminic glycans, some of them being sialylated or fucosylated (Baudin et al, 1988). Moreover, the fractionation of ACE glycans has shown at least two types of oligosaccharides, one being rich in mannose and with one fucose residue, the another being rich in sialic acid (unpublished data). In the former study, we also demonstrated that the ACE molecule is clearly elongated in aqueous solution. It could be then hypothesized that deglycosylation would modify the ACE conformation leading to a decrease in its size. Therefore, we compared the ACE Stokes radius (Rs) before and after endoglycosidase F 2 digestion. By plotting the Rs of standard globu566 lar proteins versus (-log Kav)1/2, Kav being the constant of diffusion available on Superose 12 HPLC, ACE Rs was found to be 6.0 ±0.2 run for the native enzyme as well as for deglycosylated ACE which does not support the postulated hypothesis (Figure 2). Nevertheless, the glycans could be important for the hydrosolubility of ACE and for its stability in aqueous solution. Effect of deglycosylation on IEF pattern of ACE As judged on IEF, with Coomassie blue staining or specific zymography, ACE pi was 4.5-4.8 with 4-5 bands focused in the enzymatically active area. The deglycosylation of ACE by endoglycosidase F 2 or its desialylation by neuraminidase led to a shift of ACE pi from 4.5-^.8 to 5.0-5.3, both still with microheterogeneity as judged on protein staining and the same displacement on zymography (Figure 3). These results obviously show that the acidic pi of ACE is partly related to its sialic acid content, the residual acidity being due to dicarboxylic amino acids since they are preponderant in pig lung ACE (Baudin et al, 1988) as well as in other species (Das et al, 1975; B6neteau-Burnat et al., 1994). Deglycosylation and desialylation increased the ACE pi almost identically, which indicates that, within ACE sugar moiety, only N-acetylneuraminic acid provides electric charges. Moreover, the Glycosyiations of angjotensln-converting enzyme maintenance of microheterogeneity after deglycosylation shows that it is not related to heterogeneity in ACE glycans, but to abnormalities in the primary sequence or to the existence of modified amino acids. Effect of deglycosylation on ACE affinity for lectins Pulmonary ACE interacted strongly with concanavalin A as shown by its complete binding onto ConA-Sepharose 4 B and by the incomplete elution from the column using ot-methylmannoside alone. A more complete elution was achieved in 0.2 M a-methylmannoside plus 0.5 M NaCl (Figure 4). In contrast, ACE binding on WGA-Ultrogel was incomplete and specific elution in 0.2 M N-acetylglucosamine was easy. Endoglycosidase F2-treated ACE did not bind onto either of the lectins, demonstrating the role of ACE glycans in the interactions with these lectins. These data are in favor of the predominance in pulmonary ACE of oligomannosidic or hybrid structures. Fig. 2. Plot of Stokes radius in run (Y) versus (-log Kav)'« (X), Kav being measured on Superose 12 HPLC. •, Rs standards; O, native ACE; A, endoglycosidase F2-treated ACE. .B- -A. 2.8 • 3.75 • 4.15 • 4.55 • 5.2 • Effect of deglycosylation on ACE catalytic activity ACE activity was radiometrically determined on synthetic substrate; neither endoglycosidase F 2 - nor N-glycanase-treatment significantly modified ACE kcat in comparison with native pH in situ 3L 5.5 5.85 • 6.55 »* 6 8 9 10 Fig. 3. IEF of pig lung ACE before (2, 8) and after desialylation by neuraminidase (3, 4, 9) or after deglycosylation by endoglycosidase F2 (5, 6, 10). pi standards (1, 7). 2, 4, 5: 20 p.g of ACE; 3, 6, 8, 9, 10: 10 (ig of ACE. Coomassie blue staining (A) and specific ACE zymography (B). 367 B.Baudin et al WGA CON-A 0.05 _ £ £ 0 £ CM b I o aci 280 z £ 6 • ro z 1 AI £ M 1 0.01 _ 40 10 I 10 30 ml 0.0 5 I B I 0.01 10 40 30 ml Fig. 4. Chromatography on agarose-bound lectins of pig lung ACE before (A) and afteT endogtycosidase F2-treatment (B). OLMM, a-methylmannoside; GN, N-acetylglucosamine. All protein peaks contained ACE activity. 568 GlycosyUtions of angiotensin-converting enzyme ACE incubated in the respective buffers but without the glycosidases (Table I). These results correlate with those of IEF where ACE zymography was possible even after the deglycosylations, but not after N-glycanase treatment after denaturation of ACE which completely abolished its activity. Nevertheless, desialylation decreased ACE kcat by 30% without clear explanation. Thus, ACE glycans do not seem indispensable for its enzymatic activity, although sialic acid could have a significant importance on the catalytic events in ACE active site. Table IL Effect of tunicamycin on ACE biosynthesis and secretion by porcine pulmonary artery endothelial cells: incubation with (+) or without (-) 10 jig/ml tunicamycin Culture supernatant (U/ml) Cells (U/mg proteins) 24 h 0.523 ± 0.09* 2.197 ±0.48 NS b NS 2.129 ±0.32 0-506 ±0.10 48 h Effect of tunicamycin on ACE biosynthesis and secretion by endothelial cells Endothelial cells were grown in vitro from the pig pulmonary artery; 48 h after confluency, i.e., when the expression of ACE is maximal (Baudin et al., 1996), primary cultures were incubated for 24 or 48 h with 10 u-g/ml tunicamycin, an inhibitor of cellular N-glycosylation. This treatment did not modify ACE secretion in the culture medium or its cellular biosynthesis since ACE activity in both media did not vary (Table II). A higher tunicamycin concentration was toxic for the cells, therefore we could not be sure that tunicamycin completely blocked N-glycosylation. However, glycosylation of endothelial ACE does not seem important for its secretion by the endothelium. It is noteworthy that glycans are indispensable for testicular ACE since the blockage of glycosylation results in rapid intracellular turnover of the underglycosylated protein (Kasturi et al., 1994). On the other hand, intact glycosylated chains are necessary for thrombospondin secretion by human endothelial cells (Vischer et al., 1985). Nevertheless, ACE glycans could be important in its intracellular targeting, in particular for the expression of the membrane-bound form and the secretion of the soluble form, maybe also for the protection of the soluble form against hepatic clearance, since ACE contains both galactose and sialic acid residues; some of them could be exposed so as to recognize endogeneous lectins. Materials and methods Reagents ACE was purified to electropboretic homogeneity from pig lung using a protocol that we have previously detailed (Baudin et aL, 1991). Endoglycosidase F 2 (endo-P-N-acetylglucosaminidase F 2 , EC.3.2.1.96) from Flavobacterium meningosepticum, and recombinant N-glycanase (peptide: N-glycosidase F, EC.3.5.1.52) were from Genzyme (Cambridge, MA). Neuraminidase (acetylneuraminylhydrolase, EC.3.2.1.18) from Clostridium perfringens was provided by Sigma (St. Louis, MO). Recombinant endoglycosidase H (EC.3.2.1.96) was from Oxford (Abingdon, UK). N-Acetylglucosamine, a-methylmannoside, Nonidet P-40, Triton X-100, phenylmethylsulfonyl fluoride (PMSF), N-ethylmaleinimide (NEM), ophthaldialdehyde, and tunicamycin were from Sigma. Dithiothreitol (DTT) and sodium dodecyl sulfate (SDS) were from Bio-Rad (CA). All other reagents of analytical grade were provided by Merck (Darmstadt, Germany) or Prolabo (Paris, France). 0.510 ±0.05 1.09 ±0.26 NS 0.526 ± 0.08 NS 1.25 ±0.26 •Mean ± SD (n = 5). "T^S, nonsignificant (p > 0.05), Mann-Whitney U test Gtycosidases digestion Endoglycosidase F 2 was used at 5 mU per mg of purified ACE in 0.3 M Na citrate/phosphate, pH 5.6 buffer with 1% Nonidet P^M), 1 mM PMSF and at 37°C. Endoglycosidase H was used in the same conditions but with 0.9 M Na-citrate/phosphate, pH 5.2 buffer. N-Glycanase was used at 37°C and at 17 U per mg of ACE in 0.05 M Tris, 0.1 M NaCl, pH 8 buffer plus 1% Nonidet P^40, 1 mM PMSF, and 2 mM NEM. All these enzymes were also tested after denaturation of ACE (5 min at 100°C) in 0.5% SDS and 50 mM DTT. Neuraminidase digestion was carried out at 37°C, at 10 U per mg of ACE, in 0.05 M Na-citrate/phosphate, 20 mM CaCl2, 1 mM PMSF, 2 mM NEM, pH 5.6 buffer. After enzymatic hydrolysis, the solutions were dialyzcd in Microdialyzer System 500 from Pierce (Rockford, IL) (cut-off 1000 Da) against 0.05 M Tris, 0.1 M NaCl, pH 8 buffer. Electrophoresis Sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE) was performed on 6.5% gels using Bio-Rad materials, dithiothreitol as a reducing reagent and followed by Coomassie blue R-250 staining. Gels were calibrated for molecular mass (MJ determination using SDS-PAGE standards "High Molecular Weight" from Bio-Rad. Isoelectric focusing was carried out on LKB system (Pharmacia, Uppsala, Sweden) in the pH range 4.0-6.5 (2.2% Ampholine); ACE was revealed by both Coomassie blue staining and a specific fluorimetric zymogram which we have developed from the method of Friedland and Silverstein (1976) using hippuryl-histidyl-leucine as the substrate (Bachem, Bubendorf, Switzerland) and o-phthaldialdehyde to promote the fluorescence of histidyl-leucine (Baudin et aL, 1986). Gels were calibrated for isoelectric point (pi) determination using the low pi isoelectric focusing calibration kit from Pharmacia; the pH was also measured in situ using a Microprocessor Ionalyser model 901 from Orion Research (Mettler, France). Ckromatography Size-exclusion HPLC was performed on Superose 12 HR 10/30 column, from Pharmacia, calibrated with gel-filtration standards, from Bio-Rad, and using Gilson material as previously described (Baudin et aL, 1991). Lectin-affinity chromatography was carried out in 2 ml columns fitted with either Concanavalin A-Sepharose 4 B (Pharmacia) or wheat germ agglutinin-Ultrogel (Biosepra, ViUeneuve-la-Garenne, France), at 15 ml/h and in 0.1 M sodium phosphate, 0.1 M NaCl, 1 mM CaCl2, 1 mM MgCl2, 1 mM MnCl2, pH 7.4 buffer. Culture of endothelial celts Table I. Effect of glycosidase treatment on ACE catalytic activity as judged on the hydrolysis of hippuryl-histidyl-leucine Control* Glycosidase N-Glycanase EndoF2 Neuraminidase 19.4 9.8 9.1 9.8 6.8 •Native ACE dissolved in the respective buffers, then dialyzed like for the aliquots treated by the glycosidase. b In units per mg of protein (kcat), mean of three determinations. Endothelial cells were cultured from pig pulmonary arteries according to a method which we have previously detailed (Baudin et aL, 1996). Primary cultures only were used. After reaching perfect confluency, the cells were rinsed and incubated with 1 ml of serum-free medium containing 0 to 10 M-g/ml tunicamycin, for 24 or 48 h, at 37°C in 5% CO 2 , 95% air atmosphere. Culture supernatants were collected at the end of the incubation; they contained ACE secreted by the cell monolayers in the time interval. Then the monolayers were washed twice with serum-free medium and were lysed for 15 min at 37°C with 1% Triton X-100 in phosphate-buffered saline containing 2 mM PMSF and 5 mMNEM. 569 B.Baudin et aL ACE assay l4 ACE activity was radiometrically determined using ( C-glycine)hippurylhistidyl-leucine (New England Nuclear, Boston, MA) in an assay that we previously developed (Baudin et aL, 1990). Enzyme activity is expressed as micromoles of substrate hydrolyzed per minute per milligram of protein, ACE protein being measured using e ^ ^ , = 1.5 x 105 M~' cm"1 calculated on UV-spectrum (Baudin et aL, 1995), and total proteins in cell lysates using Markwell's method (1978) based on Lowry's reaction but avoiding the interference due to the detergent which is still in the cell extracts. Acknowledgments We thank Ms. Pascale Jue for the perfect typing of the manuscript and Paul Fradet for taking photographs of the gels. 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(1975) Subcellular localization of pulmonary angiotensin-converting enzyme (kininase II). Biochem. J., 146, 497-499. Soubrier,F., Alhenc-GeUs,F., Hubert,C, AllegriniJ., JohruM., Tregear.G. and CorvolJ1. (1988) Two putative active centers in human angiotensin Iconverting enzyme revealed by molecular cloning. Proc. NatL Acad. ScL USA, 85, 9386-9390. Vischer,P., Beeckji. and Voss3. (1985) Synthesis, intracellular processing and secretion of thrombospondin in human endothelial cells. Eur. J. Biochem., 153, 435-443. Received on September 18, 1996; revised on October 22, 1996; accepted on October 22, 1996
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