Physarum polymalic acid hydrolase: Recombinant expression and enzyme activation
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Biochemical and Biophysical Research Communications 377 (2008) 735–740
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Biochemical and Biophysical Research Communications j o u r n a l h o m e p a g e : w w w . e l s e v i e r. c o m / l o c a t e / y b b r c
Physarum polymalic acid hydrolase: Recombinant expression and enzyme activation Wolfgang Mueller, Markus Haindl, Eggehard Holler * Biophysik und Physikalische Biochemie, Universitaet Regensburg, 93040 Regensburg, Germany
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Article history: Received 12 September 2008 Available online 7 October 2008 Keywords: Recombinant expression in Escherichia coli and yeast Glycosylation Zymogen Hydrolase activation by phosphorylation Plasma membrane protein tyrosine kinase Secretion Membrane damage Plasmodium physiology Biotechnology Nanoconjugates
a b s t r a c t As a platform for syntheses of nanoconjugates in antitumor drug delivery, polymalic acid together with its tailoring specific exohydrolase is purified from plasmodium cultures of the slime mold Physarum poly cephalum, a member of the phylum myxomycota. Polymalic acid hydrolase is expressed in an inactive form that functions as a molecul ar adapter for polymalic acid traffi cking within the plasmodium and is activated only during secretion. Activation follows specific protein tyrosine phosphorylation and disso ciation from plasma membranes. Purified inactive Physarum polymalic acid hydrolase, recombinantly expressed in yeast Saccharomyces, is activated on a preparative basis by the addition of plasma membrane fragments from plasmodia of P. polycephalum. Activation of polymalic acid hydrolase and inhibition of polymalic acid synthesis by protein tyrosine phosphorylation are complementary events and could indi cate a joint signal response to plasma membrane damage. © 2008 Elsevier Inc. All rights reserved.
The natural substrate of polymalic acid hydrolase (PMase) is polymalic acid [b-poly(l-malic acid), PMLA] [1]. The unique poly ester receives high interest as a molecular carrier of especially nucleic acid interacting proteins in the multinucleated giant plas modium of acellular slime molds (myxomycotae) [2–5] [and refer ences therein] and, recently, in nanomedicine as a biodegradable, nontoxic, nonimmunogenic polyfunctional platform for the syn thesis of drug delivery nanoconjugates called Polycefins [6,7 and references therein]. PMLA is highly expressed in the plasmodium of Physarum poly cephalum [8] to aid the distribution of nuclear proteins which are involved in synchronous nuclei division and cell growth [9,10]. PMLA and PMase are jointly expressed [1,4,11], and the protein, not enzymatic ally active in the cell, has been attributed the function of a molecul ar chaperone of PMLA [9,12]. PMLA is constitutively expressed [8] and engaged in mega protein complexes in nuclei and cytoplasm [9]. Surplus PMLA and the activated PMase are secreted and can be harvested and purified from the culture broth [1,12,13]. The enzyme has been characterized in detail and found to be a valuable tool for biotechnical tailoring of PMLA [1,14]. How ever, purification of the protein is extremely troublesome and does Abbreviations: PMse, polymalatase, polymalic acid hydrolase; PMLA, polymalic acid; ATCC, American type culture collection. * Corresponding author. Fax: +49 941 943 2813. E-mail address: eggehard.holler@biologie.uni-regensburg.de (E. Holler). 0006-291X/$ - see front matter © 2008 Elsevier Inc. All rights reserved. doi:10.1016/j.bbrc.2008.09.127
not allow provision of large amounts of pure enzyme. The mode of activation is unsolved, although activation by limited cleavage of a high molecular mass zymogen during secretion has been sug gested [12]. In the present communication, a method for the con trolled activation of PMase and a route for recombinant synthesis and purification will be presented. Materials and methods Protease inhibitor cocktail was bought from Roche (Basel, Switzerland). Tyrosine-specific protein-phosphatase (EC 3.1.3.48) and Tyrphostin-47 were obtained from Calbiochem (San Diego, CA) and enzymes for recombinant work from Invitrogen (Karlsruhe, Germany), Promega (Madison, WI, USA), Roche Diagnostics (Mannheim, Germany), New England Biolabs (Bad Schwalbac, Germany), and kits from Machery-Nagel (Dueren, Germany), Quiagen (Hilden, Germany), Promega (Mannheim, Germany). All other chemic als were purchased from Merck (Darmstadt, Germany). Anti-PMase antibody against key hole limpet hemocyanin (KLH)-conjugated oligopeptide NH2CA(203)GGVEHPVYPEGKWR (217)-CONH2 was custom made and affinity purified by Pineda (Berlin, Germany). Anti-His6-perox idase was from Roche Diagnostics (Mannheim, Germany) and anti-rabbit IgG-peroxid ase (2nd antibody) from Pierce (Rockford, USA). Primers for cDNA cloning were 59Nhel, 59-TAA TTA CAT GAT
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W. Mueller et al. / Biochemical and Biophysical Research Communications 377 (2008) 735–740
GCG GCC CTC TAG-39 and 39Notl 59-ATA AGA STG CGG CCG CTA GTT TGC TCA TTT CTT GG-39 and for cDNA without signal peptide 59HindIII_SP, 59-AGC TAA GCT TAA AAA TGG GAA GTG GCC CGG AAC AAA CGT TCT TC-39 and 39Strebb 59-ACG TGA ATT CTC ATT TTT CGA ACT GCG GGT GGC TCC AAG CGC TGT G-39. Plasmodia of P. polycephalum yellow, wild type, high PMLA pro ducer M3CVII (ATCC 204388) were grown as described [13]. For clon ing and recombinant expression of PMAse, the Escherichia coli strains NEB 5a, NEB T7 RP and NEB T7 Rosetta (New England Biolabs, Ips wich, MA, USA) were used and for expression in yeast Saccharomyces cerevisiae strains c13-ABYS-86 [15] and S. cerevisiae W303-1A [16]. mRNA isolation, RT-PCR and DNA-cloning. The gene of P. polyceph alum PMase comprises 2233 bp and includes a 42 bp 59-untranslated region, a hydrophobic leader peptide MHSRSACIFVLCGLLPFVLG, the coded protein sequence, and a 71 bp 39-untranslated region with a short oligo(A) tail (Gene Bank Accession No. AJ543320). Total RNA of 2 days old Physarum plasmodia was isolated with the Rneasy kit (Quiagen, Hilden, Germany) and analyzed by agarose (1%) gel electrophoresis. Transcription into cDNA was carried out with SuperScript™ III Reverse Transcriptase (Invitrogen, Karlsruhe, Germany) and Oligo dT18 primer. The PMAse coding sequence was amplified by standard PCR-methods using Phusion™ High Fidel ity Polymerase (New England Biolabs, Ipswich, MA, USA) and gene specific primers 59Nhel and 39Notl. For expression in E. coli, PCR fragments purified by agarose gel electrophoresis were digested with NheI/NotI and cloned into the pET24a(+) vector (Invitrogen) in-frame with the C-terminal His6tag. For expression in S. cerevisiae, sequences were inserted via HindIII and EcoRI in the pYES2 shuttle vector including N-termi nal Kozak translation initiat ion sequence and C-terminal His10-tag. After T4 DNA-Ligase ligation (Fermentas, St. Leon-Rot, Germany), E. coli NEB 5a (New England Biolabs) was transformed and constructs were verified by DNA sequencing at GeneArt AG (Regensburg, Ger many). S. cerevisiae strains W303 and c13 were transformed by the LiAc method [17]. Plasmid DNA from E. coli was isolated with QIA prep Spin Miniprep kit (Quiagen) and DNA fragments after agarose gel electrophoresis with QIAquick Gel Extraction kit (Quiagen). cDNA devoid of signal peptide, was PCR amplified with primers 59HindIII_SP and 39Strebb and cloned into vector pYES2. Recombinant expression. E. coli NEB T7 RP and NEB T7 Rosetta (New England Biolabs) grown at 37 °C in LB-media. Protein expres sion in 5 L was induced with 0.1 mM IPTG at an OD600 of 0.6 After 12 h at 15 °C, pelleted cells (3000g for 10 min) were resuspended in extraction buffer (Tris–HCl 100 mM, pH 7.5, KCl 300 mM, PMSF 1 mM, imidazole 10 mM) and sonicated (Branson sonifier, Heinemann, Hamburg, Germany). After centrifugation at 20,000g for 20 min at 4 °C, soluble cell extract was subjected to Ni-chelate chromatography. Saccaromyces cerevisiae W303 or c13 was grown at 30 °C in SD-medium without uracil containing 2% glucose until an OD600 of 0.8. Cells pelleted at 3000g for 10 min were suspended in 5 L of induction medium containing 2% galactose. After 12 h at 30 °C, pelleted cells were suspended in extraction buffer and lysed with glass beads equipped disrupter (Fritsch, Idar-Oberstein, Germany). Cell fragments and nuclei were pelleted at 3000g for 15 min at 4 °C before cell membranes were sedimented at 20,000g for 20 min. Pellet after 2 h treatment at 4 °C with extraction buffer, 2% (v/v) Tri ton X100 was centrifuged at 20,000g for 20 min, and PMase puri fied by Ni-chelate chromatography. Preparation of Physarum crude membrane suspension. Plasmo dia (grown for 2d) harvested on a nylon sieve was washed three times with 25 mL portions of fresh culture medium. Portions of 2 g plasmodia were lysed at 4 °C during 8–10 strokes in a Dounce homogeniser suspended in 3 mL ice-cold extraction buffer (50 mM Tris–HCl, pH 7.5, 50 mM EGTA, 14 mM 2-mercaptoethanol, 10 mM MgCl2, 300 mM NaCl, protease inhibit or cocktail, and 20% glycerol).
After pelleting at 1000g for 15 min at 4 °C, post nuclear supernatants were again pelleted at 20,000g for 20 min yielding the membrane and the cytoplasmic fractions. Membranes were resuspended in 2 mL extraction buffer on ice. Plasma membranes were purified by isopycnic sucrose gradient centrifugation [18]. Fractions starting from the bottom were assayed for PMase and alkaline phosphatase (plasma membrane marker) activities. Purification of recombinant protein. Soluble cell extract was loaded on a 1 ml Ni2+-charged HisTrap FF column (4 °C, Äkta Prime System, GE Healthcare, Munich, Germany) and washed with 100 mM Tris–HCl (pH 7.5), 300 mM KCl, 10 mM imidazole, and PMase eluted with 100 mL linear 10 mM–500 mM imidazole gradi ent between 50 mM and 150 mM imidazole. After dialysis against 50 mM Tris–HCl (pH 7.5), the purified protein was concentrated in a Centricon (Billerica, MA, USA) (15 mL). PMase activation, enzyme assays and other methods. Recombinant PMase was activated in a mixture of 0.5 mL activation buffer, 20–500 nM purified recombinant PMase, 2% Triton X100, 2 mM MgATP, and 50 lL purified membranes (suspension of membranes from 2 g Physarum plasmodia) at 20 °C for various times. After 20 min centrifugation at 20,000g, 20 lL aliquots were assayed for PMase activity and/or analyzed by SDS–PAGE—Western blotting (PMase antibody). Background activity of membranes was mea sured in absence of recombinant PMase-protein and subtracted from total activity. The size of the activation reaction mixture could be easily upscaled. PMLA and activity of PMase were measured as described [12]. PMase activity refers to A340-units £ h¡1 of NADH in the stan dard (malate dehydrogenase) assay equivalent to the amount of l-malate. Purified PMase, PMase-His6-tag, PMase-His10-tag, PMase-Streptag, and PMase(devoid of signal peptide) were quantitated using the specific absorbencies 0.1%A280 [cm2 mg¡1] of 1.513, 1.497, 1.486, 1.544, and 1.555. SDS–PAGE, Western blotting with luminescence detection followed a manufacturer’s protocol http://www.ener gene.com/products.htm#NOWA. For incorporation of 32P, mixtures of 100 lL membranes in activation buffer with 5 lCi of either [a-32P]ATP (3000 Ci/mmol, Amersham) or [c-32P]ATP (5000 Ci/mmol) were incubated 15 min at 25 °C and analyzed by SDS–10%PAGE and autoradiography. Results and discussion Syntheses of recombinant PMAse-protein First tests of recombinant synthesis were carried out with E. coli. PMase-protein expressed in E. coli NEB T7 RP and NEB T7 Rosetta, was detected in pellets and supernatants (Fig. 1). By Western blotting with PMase-specific antiserum (Fig. 1A) several protein bands and by blotting with anti-His-tag antibody a single protein (Fig. 1B) revealed a polypeptide of 75 ± 2 kDa degraded from the C-terminal His-tag. The protein was purified from the soluble fraction (2 mg from 5 L induction medium, OD600 = 1.0), and was enzymatically inactive. In principle, recombinant syn thesis was feasible, but because of fragmentation this route was not followed. Saccharomyces cerevisiae strains W303 and c13 were useful. The degree of fragmentation was acceptable in strain c13, used further on. His6-tag was replaced by His10-tag or Strep-tag to reduce copu rification of yeast proteins (Fig. 1C and D). PMase-protein was con tained in particulate fractions and solubilized on standing. After extraction with 2% Triton X100 (lane MS in Fig. 1F), soluble PMseprotein was purified by Ni-chelate chromatography (3.5 mg from 5 L induction medium, OD600 = 1). The molecular mass 92 ± 2 kDa was the same for pellet and supernatant and higher than that of E. coli recombinant protein (75 ± 2 kDa) but less than 97 ± 2 kDa for P.
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Fig. 1. Recombinant expression of PMase-protein in Escherichia coli and yeast. (A) Expression of PMase in E. coli NEB T7 RP and NEB T7 Rosetta after induction with 0.1 mM IPTG. Lane P, pellet; lane S, supernatant. Western blot (SDS–12.5%PAGE) with anti-PMase antibody. (B) Same as a, but detection with anti-His6 antibody. (C) Purification of Saccharomyces cerevisiae c13 recombinant PMase-His10 by Ni-chelate affinity chromatography. Lane C, crude cell extract; lane X, column break-through, lanes 13–23, peak elution; lane St, molecular mass standards (SDS–8%PAGE, Coomassie Brillant Blue staining). (D) Purification of yeast recombinant PMAase-protein-Strep by StrepTactin chro matography; lane W2 and W5, column wash; lanes E1–E8 peak elution (SDS–8%PAGE, silver staining). (E) Yeast recombinant PMase truncated from signal peptide. Lane K, non-truncated PMase; lane MP, truncated PMase in the membrane pellet; lane S, truncated PMase in the supernatant. (F) Yeast was unable to secrete recombinant PMaseprotein as shown in lane K for concentrated sample of culture broth after ammonium sulfate precipitation. Yeast recombinant PMase is shown in fractionated cell extracts: Lane C, yeast crude extract. lane P1, pellet after low speed centrifugation; lane S, supernatant after a second, high speed centrifugation in the absence of Triton X100, and the corresponding pellet in lane P2. This pellet was extracted in the presence of 2% Triton X100 in lane MS. Western blots (SDS–8%PAGE, PMase antibody) were prepared with 5 lL of 10-fold diluted samples.
polycephalum. Molecular mass was 75 kDa when the leader peptide was truncated (yeast PMase), and identical with PMase expressed by E. coli (Fig. 1A, B and E, lanes S, MP). Although recombinant PMase was glycosylated, it was not secreted into the culture broth (no detection even after concentration by 65% ammonium sulfate precipitation, lane K, Fig. 1F). The recombinant PMase was not enzymatic ally active.
In search of PMase activation Distribution of endogenous PMase-protein As with E. coli and yeast, PMase of P. polycephalum was con tained in the particulate and its release during standing was increased in the presence of 2% Triton X100 (Fig. 2). At variance
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Fig. 2. PMase activation by solubilization. (A) PMase activity in fractions of plasma membranes purified by isopycnic 30–65% sucrose gradient centrifugation [18]. Activities of PMase and inorganic phosphatase (marker for plasma membranes) fractionate together. (B) Solubilized PMase-protein by Western blotting (anti-PMase antibody) appeared on standing of plasma membranes in the supernatant together with hydrolase activity. (C) The same experim ent as in figure b in the presence of 2% Triton X100. (D and E) Spontaneous fragmentation of PMase in extracts and culture broth of 2 and 3 days old plasmodia. Lane B, culture broth; lane P1, pellet containing nuclei and cell fragments; lane P2, membrane pellet; lane S1, supernatant of membrane pellet; lane E, crude extract. (F) PMase activity appeared in the supernatants of panel B (no Triton X100) and C (2% Triton X100). Means and standard deviations refer to experiments in triplicates.
with yeast, released protein was enzymatically active, and the culture broth of Physarum contained enzymatic ally active PMase [1,12]. When Physarum plasma membrane was purified by iso pycnic centrifugation, PMase fractionated together with inor ganic phosphatase, a marker for plasma membranes (Fig. 2A). The purified membrane fraction itself was devoid of hydrolase activity, however, on standing, PMase activity appeared together with solubilized PMase-protein (Fig. 2B and F), and increased in the presence of 2% Triton X100 (Fig. 2B, C, and F). The results suggested that PMase-activase was a constitue nt of the plasma membrane. The enzymatic nature of Physarum activase Because Physarum PMAse-protein was rapidly cleaved under a variety of conditions (Fig. 2D and E), activation was at first con sidered the result of a peptide cleaving activase [12], but then was
considered unlikely after finding the activation resistant to prote ase inhibitors (data not shown). Damage of plasma membranes is known to inhibit in vivo syn thesis of PMLA by protein phosphorylation [19]. On that basis, the idea was born that phosphorylation activated PMLA degradation in a complementary fashion. To test whether a kinase was acti vase, purified Physarum plasma membranes were incubated with 2 mM MgATP and the supernatant assayed for PMase activity (Fig. 3A and B). Hydrolase activity appeared several-fold over the back ground by the membranes alone (Fig. 3A) and Triton X100 had an activating effect (Fig. 3B). The results in Fig. 3A inset ruled out that MgATP increased activation via solubilization. The activation was inhibited by Tyrphostin-47, a protein tyrosine-kinase inhibitor, or by tyrosine-specific protein-phosphatase. The results suggested activation by a membrane bound protein tyrosine kinase. Hydrolase activity unfolded only after dissocia tion of activated PMase from the membrane. Background activity
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W. Mueller et al. / Biochemical and Biophysical Research Communications 377 (2008) 735–740
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Fig. 3. PMase activation by phosphorylation. Endogenous and recombinant PMase were activated in the presence of suspended Physarum membranes. Ingredients were 2 mM MgATP, and as indicated: 2% Triton X100, 10 lM Tyrphostin-47, 40 lg/mL Tyr-phosphatase. (A) Emerging activity of endogenous PMase on standing of plasma membranes prepared by isopycnic sucrose gradient centrifugation. Figure inset shows solubilized PMase in the presence of Triton X100 or MgATP (Western with anti-PMase antibody). (B) Emerging PMase activity on standing of crude membranes in the presence of Triton X100. (C) Emerging PMase activity of yeast recombinant PMase on top of endogenous PMase (background activation) during standing in the presence of added Physarum membranes. Background activation is shown in the absence of recombinant PMase with or without bovine serum albumin (BSA). Triton X100 was present except where indicated. Average values and standard deviations refer to measurements in triplicates. Figure inset shows 32P-incorporation into proteins of purified plasma membranes after reaction with [a-32P]ATP (lane a) or [c-32P]ATP (lane b).
by solubilization was explained by in loco activation of membrane bound PMase-protein during particulate preparation. Activation of recombinant PMAase The results obtained for Physarum PMAse suggested the method for recombinant protein activation. This was born out in Fig. 3C showing activity proportional to added amounts of puri fied recombinant PMAse-protein that could not be substituted by bovine serum albumin (BSA). The net activity for 500 nM added recombinant PMAse-protein corresponded to a specific hydrolase activity of 560 U/mg comparing with 540 U/mg activity for PMAse
isolated from culture broth [1]. Reaction of Physarum membranes with [c-32P]MgATP indicated phosphorylation of a 97 kDa protein (Fig. 3C, inset), while this was not observed with [a-32P]ATP ruling out adenylation. Recombinant expression and controlled PMase activation allow preparation of active enzyme for biotechnical application such as nanoconjugate tailoring and provide experimental means to validate supposed in vivo functions of PMase and PMLA thereby advancing knowledge about the physiology of plasmodia. Emerging is the role of protein tyrosine kinase in regulating synthesis and degradation of PMLA under the control of plasma membrane dam age [19]. In this context, activation of Physarum transglutaminase
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is mentioned that involves Ca2+ [20]. The second messenger could downregulate PMLA via activating tyrosine protein kinase(s). Acknowledgment The interest and support by Dr. Reinhard Sterner, Institut fuer Biophysik und Physikalische Biochemie der Universitaet Regens burg, Germany, is greatly acknowledged. References [1] C. Korherr, M. Roth, E. Holler, Poly(b-l-malate) hydrolase from plasmodia of Physarum polycephalum, Can. J. Microbiol. 41 (1995) 192–199. [2] H. Fischer, S. Erdmann, E. Holler, An unusual polyanion from Physarum poly cephalum that inhibits homologous DNA polymerase alpha in vitro, Biochem istry 28 (1989) 5219–5226. [3] T. Göttler, E. Holler, Screening for beta-poly(l-malate) binding proteins by affinity chromatography, Biochem. Biophys. Res. Commun. 341 (2006) 1119– 1127. [4] K. Rathberger, H. Reisner, B. Willibald, H.-P. Molitoris, E. Holler, Comparat ive synthesis and hydrolytic degradation of b-poly(l-malate) by myxomycetes and fungi, Mycol. Res. 103 (1997) 513–520. [5] B.-S. Lee, M. Vert, E. Holler, Water-soluble aliphatic polyesters: poly(malic acid)s, in: Y. Doi A. Steinbüchel (Eds.), Biopolymers, Wiley-VCH, Weinheim, 2002, pp. 75–103. [6] B.-S. Lee, M. Fujita, N.M. Khazen on, K.A. Wawrowsky, S. Wachsmann-Hogiu, D.I. Farkash, K.L. Black, J.Y. Ljubimova, E. Holler, Polycefin, a new prototype of multifunctional nanoconjugate based on poly(beta-l-malic acid) for drug delivery, Bioconjug. Chem. 17 (2006) 317–326. [7] J.Y. Ljubimova, M. Fujita, A.V. Ljubimov, V.P. Torchilin, K.L. Black, E. Holler, Poly(malic acid) nanoconjugates containing vario us antibodies and oligo nucleotides for multitargeting drug delivery, Nanomedicine 3 (2008) 248– 265. [8] A. Schmidt, C. Windisch, E. Holler, Nuclear accumulation and homeostasis of the unusual polymer b-poly(l-malate) in plasmodia of Physarum polyceph alum, Eur. J. Cell Biol. 70 (1995) 373–380.
[9] B. Angerer, E. Holler, Large complexes of b-poly(l-malate) with DNA polymer ase, histones, and other proteins in nuclei of growing plasmodia of Physarum polycephalum, Biochemistry 34 (1995) 14741–14751. [10] M. Karl, R. Anderson, E. Holler, Injection of poly(b-l-malate) into The plas modium of Physarum polycephalum shortens the cell cycle and increases the growth rate, Eur. J. Biochem. 271 (2004) 3805–3811. [11] N. Pinchai, B.-S. Lee, E. Holler, Stage specific expression of poly(malic acid)affiliated genes in the life cycle of Physarum polycephalum. Spherulin 3b and polymalatase, FEBS J. 273 (2006) 1046–1055. [12] M. Karl, E. Holler, Multiple polypeptides immunologically related to b-poly(lmalate) hydrolase (PMase) in the plasmodium of the slime mold Physarum polycephalum, Eur. J. Biochem. 251 (1998) 405–412. [13] B.-S. Lee, E. Holler, Effects of culture conditions on b-poly(l-malate) produc tion by Physarum polycephalum, Appl. Microbiol. Biotechnol. 51 (1999) 647– 652. [14] B. Gaßlmaier, E. Holler, Specificity and direction of depolymerization of b-poly(l-malate) catalysed by polymalatase from Physarum polycephalum. Fluorescence labeling at the carboxy-terminus of b-poly(l-malate), Eur. J. Bio chem. 250 (1997) 308–314. [15] W. Heinemeyer, J.A. Kleinschmidt, Proteinase yscE, the yeast proteasome/mul ticatalytic-multifunctional proteinase: mutants unravel its function in stress induced proteolysis and uncover its necessity for cell survival, EMBO J. 10 (1991) 555–562. [16] B.J. Thomas, R. Rothstein, Elevated recombination rates in transcriptionally active DNA, Cell 56 (1989) 619–630. [17] C. Guthrie, G.R. Fink, Guide to yeast genetics and molecular biology, Methods Enzymol. 194 (1991) 1–863. [18] D. Pallotta, A. Barden, R. Martel, J. Kiruac-Brunet, F. Bernier, A. Lord, G. Lem ieux, Plasma membranes from Physarum polycephalum plasmodia: purifica tion, characterization, and comparison with amoebae plasma membranes, Can. J. Biochem. Cell Biol. 62 (1984) 831–836. [19] B. Willibald, W. Bildl, B.-S. Lee, E. Holler, Is b-poly(l-malate) synthesis cata lysed by a combination of b-l-malate-AMP-ligase and b-poly(l-malate) poly merase?, Eur. J. Biochem. 265 (1999) 1085–1090. [20] F. Wada, H. Hasegawa, A. Nakamura, Y. Sugimura, Y. Kawai, N. Sasaki, H. Shi bata, M. Maki, K. Hitomi, Identification of substrates for transglutaminase in Physarum polycephalum, an acellular slime mold, upon cellular mechanical damage, FEBS J. 274 (2007) 2766–2777.
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