Abstract
It is generally accepted that the primary specificity of metallocarboxypeptidases is mainly determined by the structure of the so–called primary specificity pocket. However, the G215S/A251G/T257A/D260G/T262D mutant of carboxypeptidase T from Thermoactinomyces vulgaris (CPT) with the primary specificity pocket fully reproducing the one in pancreatic carboxypeptidase B (CPB) retained the broad, mainly hydrophobic substrate specificity of the wild–type enzyme. In order to elucidate factors affecting substrate specificity of metallocarboxypeptidases and the reasons for the discrepancy with the established views, we have solved the structure of the complex of the CPT G215S/A251G/T257A/D260G/T262D mutant with the transition state analogue N–sulfamoyl–L–phenylalanine at a resolution of 1.35 Å and compared it with the structure of similar complex formed by CPB. The comparative study revealed a previously underestimated structural determinant of the substrate specificity of metallocarboxypeptidases and showed that even if substitution of five amino acid residues in the primary specificity pocket results in its almost complete structural correspondence to the analogous pocket in CPB, this does not lead to fundamental changes in the substrate specificity of the mutant enzyme due to the differences in the structure of the mobile loop located at the active site entrance that affects the substrate–induced conformational rearrangements of the active site.
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Abbreviations
- BSA:
-
buried surface area
- CPB:
-
carboxypeptidase B from porcine pancreas
- CPT:
-
carboxypeptidase T from Thermoactinomyces vulgaris
- CPT5:
-
CPT mutant with A243G, T250A, A253G, D260G, T262D substitutions
- CPTwt:
-
wild–type carboxypeptidase T
- CPU:
-
carboxypeptidase U
- CPO:
-
carboxypeptidase O
- SPhe:
-
N–sulfamoyl–L–phenylalanine
- ZAAL:
-
N–benzyloxycarbonyl–L–alanyl–L–alanyl–L–leucine
References
Perez–Silva, J. G., Espanol, Y., Velasco, G., and Quesada, V. (2016) The Degradome database: expanding roles of mammalian proteases in life and disease, Nucleic Acids Res., 44, D351–D355.
Turk, B., Turk, D., and Turk, V. (2012) Protease signalling: the cutting edge, EMBO J., 31, 1630–1643.
Turk, B. (2006) Targeting proteases: successes, failures and future prospects, Nat. Rev. Drug Discov., 5, 785–799.
Tanco, S., Tort, O., Demol, H., Aviles, F. X., Gevaert, K., Van Damme, P., and Lorenzo, J. (2015) C–terminomics screen for natural substrates of cytosolic carboxypeptidase 1 reveals processing of acidic protein Ctermini, Mol. Cell. Proteomics, 14, 177–190.
Sapio, M. R., and Fricker, L. D. (2014) Carboxypeptidases in disease: insights from peptidomic studies, Proteomics Clin. Appl., 8, 327–337.
Osterman, A. L., Stepanov, V. M., Rudenskaya, G. N., Khodova, O. M., and Tsaplina, I. A. (1984) Carboxypeptidase T–extracellular carboxypeptodase of Thermoactinomyces–a distant analogue of animal car–boxypeptidases, Biokhimiya, 49, 292–301.
Teplyakov, A., Polyakov, K., Obmolova, G., Strokopytov, B., Kuranova, I., Osterman, A. L., Grishin, N., Smulevitch, S., Zagnitko, O., and Galperina, O. (1992) Crystal structure of carboxypeptidase T from Thermoactinomyces vulgaris, Eur. J. Biochem., 208, 281–288.
Schechter, I., and Berger, A. (1967) On the size of the active site in proteases. I. Papain, Biochem. Biophys. Res. Commun., 27, 157–162.
Auld, D. S., Galdes, A., Geoghegan, K. F., Holmquist, B., Martinelli, R., and Vallee, B. L. (1984) Cryospectrokinetic characterization of intermediates in biochemical reactions: carboxypeptidase A, Proc. Natl. Acad. Sci. USA, 81, 5041–5045.
Reeke, G. N., Hartsuck, J. A., Ludwig, M. L., Quiocho, F. A., Steitz, T. A., and Lipscomb, W. N. (1967) The structure of carboxypeptidase A. VI. Some results at 2.0–Å resolution, and the complex with glycyl–tyrosine at 2.8–Å resolution, Proc. Natl. Acad. Sci. USA, 58, 2220–2226.
Gardell, S. J., Craik, C. S., Clauser, E., Goldsmith, E. J., Stewart, C. B., Graf, M., and Rutter, W. J. (1988) A novel rat carboxypeptidase, CPA2: characterization, molecular cloning, and evolutionary implications on substrate specificity in the carboxypeptidase gene family, J. Biol. Chem., 263, 17828–17836.
Stepanov, V. M. (1995) Carboxypeptidase T, Methods Enzymol., 248, 675–683.
Osterman, A. L., Grishin, N. V., Smulevitch, S. V., Matz, M. V., Zagnitko, O. P., Revina, L. P., and Stepanov, V. M. (1992) Primary structure of carboxypeptidase T: delineation of functionally relevant features in Zn–carboxypeptidase family, J. Protein Chem., 11, 561–570.
Reeck, G. R., Walsh, K. A., Hermodson, M. A., and Neurath, H. (1971) New forms of bovine carboxypeptidase B and their homologous relationships to carboxypeptidase A, Proc. Natl. Acad. Sci. USA, 68, 1226–1230.
Bunnage, M. E., Blagg, J., Steele, J., Owen, D. R., Allerton, C., McElroy, A. B., Miller, D., Ringer, T., Butcher, K., Beaumont, K., Evans, K., Gray, A. J., Holland, S. J., Feeder, N., Moore, R. S., and Brown, D. G. (2007) Discovery of potent and selective inhibitors of activated thrombin–activatable fibrinolysis inhibitor for the treatment of thrombosis, J. Med. Chem., 50, 6095–6103.
Bown, D. P., and Gatehouse, J. A. (2004) Characterization of a digestive carboxypeptidase from the insect pest corn earworm (Helicoverpa armigera) with novel specificity towards C–terminal glutamate residues, Eur. J. Biochem., 271, 2000–2011.
Edge, M., Forder, C., Hennam, J., Lee, I., Tonge, D., Hardern, I., Fitton, J., Eckersley, K., East, S., Shufflebotham, A., Blakey, D., and Slater, A. (1998) Engineered human carboxypeptidase B enzymes that hydrolyse hippuryl–L–glutamic acid: reversed–polarity mutants, Protein Eng., 11, 1229–1234.
Grishin, A. M., Akparov, V. Kh., and Chestykhina, G. G. (2008) Leu254 residue and calcium ions as new structural determinant of carboxypeptidase T substrate specificity, Biochemistry (Moscow), 73, 1140–1145.
Akparov, V. Kh., Grishin, A. M., Yusupova, M. P., Ivanova, N. M., and Chestukhina, G. G. (2007) Structural principles of the wide substrate specificity of Thermoactinomyces vulgaris carboxypeptidase T. Reconstruction of the car–boxypeptidase B primary specificity pocket, Biochemistry (Moscow), 72, 416–423.
Akparov, V. Kh., Belyanova, L. P., Baratova, L. A., and Stepanov, V. M. (1979) Subtilisin 72–a serine protease from Bac. subtilus strain 72–an enzyme similar to subtilisin Carlsberg, Biokhmiya, 44, 886–891.
Lyublinskaya, L. A., Yakusheva, L. D., and Stepanov, V. M. (1977) Synthesis of peptide substrates of subtilisin and its analogues, Bioorg. Khim., 3, 273–279.
Cueni, L. B., Bazzone, T. J., Riordan, J. F., and Vallee, B. L. (1980) Affinity chromatographic sorting of carboxypeptidase A and its chemically modified derivatives, Anal. Biochem., 107, 341–349.
Novagen pET System Manual TB055 (1997) 7th Edn., Novagen Madison, W.I.
Trachuk, L., Letarov, A., Kudelina, I. A., Yusupova, M. P., and Chestukhina, G. G. (2005) In vitro refolding of car–boxypeptidase T precursor from Thermoactinomyces vulgaris obtained in Escherichia coli as cytoplasmic inclusion bodies, Protein Expr. Purif., 40, 51–59.
Bradford, M. M. (1976) A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein–dye binding, Anal. Biochem., 72, 248–254.
Laemmli, U. K. (1970) Cleavage of structural proteins during the assembly of the head of bacteriophage T4, Nature, 227, 680–685.
Cornish–Bowden, A. (2013) Fundamentals of Enzyme Kinetics, 4th Edn., Wiley–VCH, Weinheim.
Krissinel, E., and Henrick, K. (2007) Inference of macro-molecular assemblies from crystalline state, J. Mol. Biol., 372, 774–797.
Takahashi, S., Tsurumura, T., Aritake, K., Furubayashi, N., Sato, M., Yamanaka, M., Hirota, E., Sano, S., Kobayashi, T., Tanaka, T., Inaka, K., Tanaka, H., and Urade, Y. (2010) High–quality crystals of human haematopoietic prostaglandin D synthase with novel inhibitors, Acta Crystallogr. Sect. F Struct. Biol. Cryst. Commun., 66, 846–850.
Kuranova, I. P., Smirnova, E. A., Abramchik, Yu. A., Chupova, L. A., Esipov, R. S., Akparov, V. Kh., Timofeev, V. I., and Kovalchuk, M. V. (2011) Crystal growth of phosphopantentein adenylyltransferase, carboxypeptidase T, and thymidine phosphorylase on the international space station by the capillary counter–diffusion method, Crystallogr. Rep., 56, 884–891.
McCoy, A. J., Grosse–Kunstleve, R. W., Adams, P. D., Winn, M. D., Storoni, L. C., and Read, R. J. (2007) Phaser crystallographic software, J. Appl. Crystallogr., 40, 658–674.
Murshudov, G. N., Vagin, A. A., and Dodson, E. J. (1997) Refinement of macromolecular structures by the maximum–likelihood method, Acta Crystallogr. Sect. D Biol. Crystallogr., 53, 240–255.
Emsley, P., and Cowtan, K. (2004) Coot: model–building tools for molecular graphics, Acta Crystallogr. Sect. D Biol. Crystallogr., 60, 2126–2132.
Park, J. D., Kim, D. H., Kim, S. J., Woo, J. R., and Ryu, S. E. (2002) Sulfamide–based inhibitors for carboxypeptidase A. Novel type transition state analogue inhibitors for zinc proteases, J. Med. Chem., 45, 5295–5302.
Akparov, V. K., Sokolenko, N., Timofeev, V., and Kuranova, I. (2015) Structure of the complex of carboxypeptidase B and N–sulfamoyl–L–arginine, Acta Crystallogr. Sect. F Struct. Biol. Cryst. Commun., 71, 1335–1340.
Akparov, V. Kh., Timofeev, V. I., Maghsoudi, N. N., and Kuranova, I. P. (2017) Three–dimensional structure of porcine pancreatic carboxypeptidase B with an acetate ion and two zinc atoms in the active center, Crystallogr. Rep., 62, 249–253.
Akparov, V., Timofeev, V., Khaliullin, I., Švedas, V., and Kuranova, I. (2018) Structure of the carboxypeptidase B complex with N–sulfamoyl–L–phenylalanine–a transition state analog of non–specific substrate, J. Biomol. Struct. Dyn., 36, 956–965.
Akparov, V., Timofeev, V., Khaliullin, I., Švedas, V., Kuranova, I., and Rakitina, T. (2017) Crystal structures of carboxypeptidase T complexes with transition–state analogs, J. Biomol. Struct. Dyn., 35, 1–9.
Aloy, P., Companys, V., Vendrell, J., Aviles, F. X., Fricker, L. D., Coll, M., and Gomis–Ruth, F. X. (2001) The crystal structure of the inhibitor–complexed carboxypeptidase D domain II and the modeling of regulatory carboxypeptidases, J. Biol. Chem., 276, 16177–16184.
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Originally published in Biochemistry (Moscow) On–Line Papers in Press, as Manuscript BM18–165, November 12, 2018.
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Akparov, V.K., Timofeev, V.I., Khaliullin, I.G. et al. Mobile Loop in the Active Site of Metallocarboxypeptidases as an Underestimated Determinant of Substrate Specificity. Biochemistry Moscow 83, 1594–1602 (2018). https://doi.org/10.1134/S0006297918120167
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DOI: https://doi.org/10.1134/S0006297918120167