Metabolite Channelling and Metabolic Complexity Substrate channelling in 2-0x0 acid dehydrogenase multienzyme complexes Richard N. Perharn', D.Dafydd Jones2,Hitesh J. Chauhan and Mark J. Howard3 Cambndge Centre for Molecular Recognition, Department of Biochemistry, University of Cambridge, 80 Tennis Court Road, Cambridge CB2 I GA, U.K. Abstract complex, the three component enzymes are pyruvate decarboxylase ( E l p ; EC 1.2.4.1), dihydrolipoyl acetyltransferase (E2p; EC 2.3.1.1 2) and dihydrolipoyl dehydrogenase (E3 ; EC 1.8.1.4) (reviewed in [1-4]). Corresponding enzymes make up the O G D H and BCDH complexes; in each case, the E l and E2 are specific for the particular 2-0x0 acid undergoing decarboxylation. E l catalyses the initial decarboxylation, utilizing thiamin diphosphate as a cofactor, and the subsequent reductive acetylation of a lipoyl group covalently attached to a lysine residue in E2. E2 catalyses the transfer of the acyl group to CoA and E3, which carries out an identical reaction in each complex and is normally the same enzyme in all three instances, concludes the process by reoxidizing the dihydrolipoyl group and regenerating the dithiolane ring at the expense of NAD+. In the P D H complex from Escherichia coli and most Gram-negative bacteria, E2p forms a cubic core consisting of 24 polypeptide chains arranged with octahedral symmetry, whereas in Bacillus stearothermophilus and most Grampositive bacteria, the E2p core is icosahedral and comprises 60 E2p chains [1,2]. E l and E3 are bound tightly but non-covalently in peripheral positions around the E2 core. The O G D H and BCDH complexes follow the same structural pattern, with E2 cores [dihydrolipoyl succinyltransferase (E20) and dihydrolipoyl branched chain acyltransferase (E2b)l of octahedral symmetry. T h e intact complexes are thus of giant size, with molecular masses of (5-10) x lo6 Da and diameters of up to 50 nm, significantly bigger than a ribosome. In this article we review some of the structural features of the 2-0x0 acid dehydrogenase complexes that are of particular relevance to the mechanisms of active-site coupling and substrate channelling in such vast catalytic machines [4]. Heteronuclear NMR spectroscopy and other experiments indicate that the true substrate of the E l component of 2-0x0 acid dehydrogenase complexes is not lipoic acid but the lipoyl domain of the E2 component. E l can recognize the lipoyllysine residue as such, but reductive acylation ensues only if the domain to which the lipoyl group is attached is additionally recognized by virtue of a mosaic of contacts distributed chiefly over the half of the domain that contains the lipoyl-lysine residue. The lipoyl-lysine residue may not be freely swinging, as supposed hitherto, but may adopt a preferred orientation pointing towards a nearby loop on the surface of the lipoyl domain. This in turn may facilitate the insertion of the lipoyl group into the active site of E l , where reductive acylation is to occur. The results throw new light on the concept of substrate channelling and active-site coupling in these giant multifunctional catalytic machines. Introduction T h e 2-0x0 acid dehydrogenase multienzyme complexes constitute a family of related enzymes that includes the pyruvate dehydrogenase (PDH), 2-oxoglutarate dehydrogenase (OGDH) and branched-chain 2-0x0 acid dehydrogenase (BCDH) complexes. They catalyse the oxidative decarboxylation of the relevant 2-0x0 acid, transferring the resultant acyl group to CoA and generating NADH in the process. In the P D H Key words: lipoic acid, lipoyl domain, protein-protein interaction, pyruvate dehydrogenase. Abbreviations used: BCDH, branched-chain 2-0x0 acid dehydmgenase; OGDH. 2-oxoglutamte dehydrogenase; E lo, 2-0x0glutarate decarboxylase; E I p. pyruvate decarboxylase; E2p, dihydrolipoyl acetyltransferase; E20, dihydrolipoyl succinyltransferase; E3, dihydrolipoyl dehydrogenase; PDH. pyruvate dehydrogenase; T,, transverse relaxation time. 'To whom correspondence should be addressed (e-mail r.n.perham@,bioc.cam.ac.uk). 'Present address: Novozymes AIS, Protein Screening, 6E2.06, Smtarmosevej I I , DK-2880 Bagsvcerd, Denmark 3Present address: Research School of Biosciences, University of Kent, Canterbury, Kent CT2 7N], U.K. The lipoyl domain and active-site coupling The lipoyl group is covalently attached in an amide linkage to the p - a m i n o group of a specific lysine residue of an independently folded domain (about 80 residues) that forms the N-terminal part 47 0 2002 Biochemical Society Biochemical Society Transactions (2002) Volume 30, part 2 side of the domain (Figure 1). Exact positioning of the target lysine within the protruding /?-turn is essential for correct post-translational modification by the lipoylating system(s) of the E. cob cell [ 121. of the E2 chain. T h e number of lipoyl domains per E2 chain can vary, e.g from one in the E2p chain of B. stearothermophilus and the E20 chain of E. coli to three in the E2p chain of E. coli [1,2]. T h e lipoyl domain plays a vital role in coupling the reactions within the complex in an organized and specific manner. Acting as a ‘swinging arm ’ [S], the lipoyllysine group visits each of the three active sites of the complex, carried by a lipoyl domain that is itself rendered mobile by virtue of the conformational flexibility in the segment of polypeptide chain that links it to the inner E2 core of the complex. T h e NMR solution structures of the single E. coli E20 [6] and the innermost of the three E. coli E2p [7] lipoyl domains have been solved, as have those of others from various other organisms [%lo], including that of the B. stearothermophilus E2p chain [ l l ] . Their overall backbone structures are virtually identical. They consist of a P-barrel formed from two four-stranded P-sheets, arranged with a 2-fold axis of quasi-symmetry. T h e lipoyllysine is located at the tip of a tight, type I /?-turn in one P-sheet, and the N- and C-termini are close in space in the other /?-sheet on the opposite Substrate channelling As shown first with the PDH complex of E. coli, free lipoate can act as the substrate for E2p and E3 but is a very poor substrate for E l p . However, the E2p lipoyl domain is an excellent substrate (kcat/&, raised by a factor of lo4); moreover, the E2p and E20 lipoyl domains from E. coli function as substrates only for their cognate E l s ([13,14] and references therein). Similar results have been reported for the lipoyl domains of Azotobacter vinelandii E2p and E20 [15]. T h u s the true substrate in these complexes is not lipoic acid or lipoyl-lysine but the lipoyl domain; recognition of the domain by its cognate E l provides an elegant mechanism for substrate channelling whereby reductive acylation is confined to a lipoyl group covalently attached to a specific lysine residue of Figure I Structure of the innermost lipoyl domain of € coli E2p Left-hand panel, schematic structure of the lipoyl domain drawn using MOLSCRIPT [23], with a freely rotating lipoyl-lysine residue at the tip of the p-turn between p-strands 4 and 5. Middle and right-hand panels, two views of the lipoyl domain with the lipoyl-lysine residue in a prefered orientation, close in space to the surface loop between B-strands I and 2. Reproduced from c/] with permission from Biochemistry 2000, 39, 8448-8459. 0 2000 Am. Chem. SOC. N-lcrm \ N-lcrm L. C-lcnn c-tcrm 0 2002 Biochemical Society 48 Metabolite Channelling and Metabolic Complexity the intended E2 component [ 2 4 ] . How the E2p and E20 lipoyl domains are recognized by their correct partner E l s yet have the same structural scaffold thus becomes an important question. thiamin diphosphate in the active site is buried at the bottom of a 2 nm-deep funnel-shaped hole at the interface between the a-and /?-subunits. In order for the lipoyl group to reach the cofactor, and assuming that no major conformational changes are involved, the protruding /?-turn housing the lipoyl-lysine residue would have to point into the entrance of the funnel and the lipoyllysine side chain (1.4 nm) to become fully extended. T h e lipoyl domain, and the surface loop region between /?-strands 1 and 2 in particular, would by necessity come into close contact with the surface of Elp, as indicated by the earlier N M R experiments [171. T h e quaternary structures of the E. coli E l p and 2-oxoglutarate decarboxylase ( E l o ; a2)and B . stearothermophilus E l p (a$,)differ, and therefore so may their interactions with the lipoyl domain. However, more detailed experiments with heteronuclear N M R spectroscopy, involving studies of both chemical shifts and transverse relaxation times (T2), have indicated that the same general principles apply [20,21]. I n the B. stearothermophilus E l p , it is clear that the incoming lipoyl domain makes contact with both E l a and El/? subunits, consistent with the active site lying between them. Moreover, although the surface loop region between /I-strands 1 and 2 is a major site of contact, there are other sites distributed Interaction of the lipoyl domain with E l T h e binding of the lipoyl domain to E . coli E l p is both weak ( K ,not less than 1 mM, despite a K , of x 20 pM) and transient [16]. Thus co-crystallization of the lipoyl domain with E l is likely to be impossible. However, N M R has been used to identify regions on the apo-form of the B. steavothermophilus E2p lipoyl domain that provide important contact sites in the interaction with E l p . A prominent surface loop, linking /?-strands 1 and 2, is present only in the /?-sheet that contains the lipoyl-lysine residue, and lies close in space to the lipoyl-lysine /?-turn (Figure 1). Alterations in chemical shift in the presence of E l indicated that this loop is likely to make contact with El during catalysis; likewise, the results of directed mutagenesis indicated that residues flanking the lipoyllysine residue in its /?-turn are also of critical importance [171. T h e crystal structures of the heterotetrameric (a$,) E l p s from Pseudomonas putida [18] and humans [19] have recently been solved. T h e Figure 2 Points of contact between the lipoylated 15coli lipoyl domain and its partner E I p Left-hand and middle panels,two views ofthe lipoyl domain rotated by I 80°,indicating residues (numbered in single-letter code) that exhibit significant changes in chemical shift in the presence of E I p. Right-hand panel, residues that exhibit significant changes in J2 values in the presence of E I p. Reproduced from [2 I] with permission. 0 (200 I) Academic Press. 4 1K (lipoyl-lysine) 41K (lipoyl-lysine) L 41K (lipoyl-lysine) 3 42A IK 49 0 2002 Biochemical Society Biochemical Society Transactions (2002) Volume 30, part 2 Given that the true substrate for the 2-0x0 acid dehydrogenase complexes is actually the lipoyl domain, much slower to diffuse than lipoic acid itself, even if free, the tethering of the lipoyl domain in the complex assumes a much clearer significance. T h e local concentration of the domain is raised to millimolar concentrations, way above the K,,, values it exhibits as a substrate for the component enzymes. Recognition of the lipoyl domain by E l provides the molecular basis of an elegant and efficient form of substrate channelling; and the flexibility in the tethering linker regions and the three-dimensional organization of the enzyme complex, together with a preferred orientation of the classical swinging arm on the surface of the domain, may promote catalytically advantageous trajectories of the domain between the contributing active sites. over the surface of the lipoyl domain physically remote from the lipoyl-lysine residue [20]. These experiments were carried out with the apodomain, as the lipoylated domain appeared to bind too tightly to the B. stearothermophilus E l p and substantial line-broadening was observed. However, with the E. coli E l p , the lipoylated domain could be studied [21], and again it was inferred that a significant number of residues on the domain, largely restricted to the lipoyl-lysinecontaining half and dominated by the lipoyl-lysine p-turn, come into contact with E l p (Figure 2). E l o did not interact detectably with the apodomain from E. coli E2p, but some interaction was detected with the holo-domain. T h e conclusion must be that the E l components can recognize the lipoyl-lysine residue as such, but that reductive acylation ensues only if the domain to which the lipoyl group is attached is additionally recognized P11. We thank the Biotechnology and Biological Sciences Research Council (BBSRC) forthe award of a research grant (to R. N.P.) and research studentships to D.D.J. and H.J.C., and the BBSRC and The Wellcome Trust for support of the core facilities of the Cambridge Centre for Molecular Recognition. W e also thank Mr C. Fuller for skilled technical assistance and numerous colleagues, in particular Dr Katherine Stott, for help and discussion. Implications for catalysis In comparing the NMR spectra of "N-labelled apo- and holo-forms of the lipoyl domain of E. coli E2p, it became apparent that the lipoyl-lysine p-turn becomes less flexible following posttranslational modification. From the chemical shift data, it appears that, rather than being freely swinging, as hitherto supposed, the lipoyl group may have a preferred orientation (Figure l ) , pointing towards the surface loop linking Bstrands 1 and 2 [7]. This is the self-same loop that comes into contact with E l as the lipoyl domain approaches the E l active site. It has also been observed that limited proteolysis of a surface loop in the E l a chain at the entrance to the active site of the E l component of the B. stearothermophilus P D H complex has a pronounced inhibitory effect on the catalytic activity of the intact complex. At the same time, there was no loss of catalytic activity of E l itself and no effect on the ability of the proteolysed E l to bring about the reductive acetylation of a free lipoyl domain [22]. This has raised the interesting possibility that the lipoyl domain may have a restricted trajectory in the intact complex, causing it to approach the E l active site in a particular way. A preferred orientation of the lipoyl-lysine residue on the lipoyl domain, directed towards the nearby surface loop between /?-strands 1 and 2, may contribute to the chance of an efficacious encounter and facilitate the insertion of the lipoyl-lysine arm into the E l active site, as discussed above. 0 2002 Biochemical Society References I 2 3 4 5 6 7 8 9 10 II 12 13 14 15 50 Reed, L. J. and Hackert, M. L. ( 1990) J. Biol. Chem. 265, 897 1-8974 Perham. R N. ( I99 I ) Biochemistry 30,850 1-85 I 2 de Kok A,, Hengeveld, A. F., Martin, A. and Westphal, A. H. ( I 998) Biochim. Biophys. A& 1385, 353-366 Perham, R. N. (2000) Annu. Rev. Biochem. 69,96 I - I004 Reed, L. J. ( I 974) Acc. Chem. Res. 7,40-46 Ricaud, P. M., Howard, M. J,, Roberts, E. L., Broadhunt, R. W. and Perham, R. N. ( 1996) J. Mol. Biol. 264, 179- I90 Jones,D. D., Stott, K. M., Howard, M. J. and Perham, R. N. (2000) Biochemistry 39, 8448-8459 Berg, A., Vervoort, J. and de Kok A. ( I 996) J. Mol. Biol. 26 I, 432442 Berg, A., Vervoort, J. and de Kok A. ( 1997) Eur. J. Biochem. 244, 352-360 Howard, M. J., Fuller, C.. Broadhurst, R. W., Perham, R. N.. Tang, J. G., Quinn, J., Diamond, A. G. and Yeaman, S. J. ( 1998) Gastroenterology I IS, I 39- I46 Dardel, F., Davis, A. L., Laue, E. D. and Perham, R. N. ( 1993) J. Mol. Biol. 229, 1037-1 048 Wallis, N. G. and Perham, R. N. ( I 994) J. Mol. Biol. 236, 209-2 I6 Graham, L. D., Packman, L. C. and Perham. R N. ( I 989) Biochemistry 28, 1574- I58 I Jones, D. D., Home, J. J., Reche, P. A. and Perham. R. N. (2000b) J. Mol. Biol. 295, 289-306 Berg, A., Westphal, A. H., Bosma. H. J. and de Kok, A. ( I 998) Eur. J. Biochem. 252, 45-50 Metabolite Channelling and Metabolic Complexity Howard, M. J., Chauhan, H. 1.. Domingo, G. J., Fuller, C. and Perham, R. N. (2000) J. Mol. Biol. 295, 1023-1 037 21 Jones,D. D., Stott. K. M., Reche, P. A. and Perham, R. N. (200 I ) J. Mol. Biol. 305, 49-60 and Perham, R. N. 22 Chauhan, H. J., Domingo, G. J.,Jung, (2000) Eur. J. Biochem. 267, 7 158-7 I 69 23 Kraulis, P. J. ( I 99 I) J. Appl. Crystallogr. 24, 946-950 Graham, L. D. and Pertlam, R. N. ( I 990) FEBS Lett. 262, 24 1-244 Wallis, N. G., Allen, M. D., Broadhurst,R. W., Lessard, I. A. D. and Perham, R. N. ( I 996) J. Mol. Biol. 263, 20 436474 kvarsson, A., Seger, K., Turley, S., Sokatch,J. R. and Hol, W. G. J. ( I 999) Nat. Struct. Biol. 6, 785-792 &arson, A,, Chuang, J. L., Wynn. R. M., Turley, S., Chuang, D. T. and Hol, W. G. J. (2000) Structure 8, Received I9 December 200 I 277-29 I Conversion of pancreatic cells to hepatocytes David Tosh', Chia-Ning Shen and Jonathan M. W. Slack Developmental Biology Programme, Department of Biology and Biochemistry, University of Bath, Bath BA2 7AY, U.K. germ layer (mesoderm, endoderm or ectoderm) [l-31. Secondly, transdifferentiation leads to a predisposition towards certain neoplastic transformations and therefore elucidating the molecular basis of the conversion will also provide information on the processes underlying the development of cancer [2]. In order to demonstrate that transdifferentiation has occurred in a system, Eguchi and Kodama [4] suggested that two prerequisites be fulfilled. T h e first involves demonstrating (preferably with molecular evidence) the differentiation state of the two cells types before and after the transdifferentiation event. T h e second prerequisite involves showing a direct ancestor-descendent relationship between the cells prior to and following transdifferentiation. It is difficult to fulfil these prerequisites under in vivo conditions. However, in vitro culture systems are more amenable to testing these prerequisites. One of the beststudied in vitro models for transdifferentiation is the conversion of pigmented epithelial cells of the retina to lens cells, so-called Wolffian lens regeneration [4]. Developing in vitro models for the transdifferentiation of one cell type to another is crucial as it will allow us to define the molecular and cellular mechanisms which distinguish the two cell types involved in the switch. Abstract Transdifferentiation is the name used to describe the conversion of one differentiated cell type to another. During development, the liver and pancreas arise from the same region of the endoderm and cells from the two organs can transdifferentiate in the adult under different experimental procedures. We have produced two in vitro models for the transdifferentiation of pancreatic cells to hepatocytes. T h e first utilizes a pancreatic exocrine cell line AR42J-B13 and the second comprises cultures of mouse embryonic pancreas. We have analysed the pancreatic hepatocytes and they express a range of liver markers including albumin, transferrin and transthyretin. We also present evidence for (i) the molecular mechanism which regulates the conversion between pancreas and liver and (ii) the cellular basis of the switch in phenotype. Introduction T h e ability of one differentiated cell type to convert to another is termed transdifferentiation or metaplasia [l-31. T h e process of transdifferentiation is important for two reasons. Firstly, for understanding the molecular and cellular basis of embryonic development, as the conversion of one cell type to another generally occurs between cells which arise from neighbouring regions of the same K e y words: C/ESPB, exocrine, glucocorticoid. liver, transdiffer- Models for the transdifferentiation of pancreas to liver entiation. Abbreviations used: HGF, hepatocyte growth factor: Dex, dexamethasone: LETF, liver-enriched transcription factor: GFP, green fluorescent protein: C/EBP, CCAAT/enhancer-binding protein. 'To whom correspondence should be addressed (e-mail [email protected]). Numerous examples of transdifferentiation exist but perhaps one of the most interesting is the appearance of hepatocytes in the pancreas. Foci of hepatocytes have been shown to be induced in the pancreas of rats, mice or hamsters following various experimental procedures, e.g. copper 51 0 2002 Biochemical Society
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