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770 FATTY ACID METABOLISM Essential fatty acids in membrane: physical properties and function CHRISTOPHER D. STUBBS* and ANTHONY D. SMITH? * Department of Pathology mid Cell Biology, Thomas Jefferson University, Philadelphia, PA 19107, U.S.A. arid t Departmerit of’C’hemicalPathology, Utiiversity College arid Middlesex School of Medicine, Loridori WII’ 6DR, U.K. The physicochemical properties of membranes are largely governed by the nature of the fatty acid components. Membrane proteins, e.g. receptors, enzymes, ion channels, etc., are highly sensitive to the lipid environment. The critical features of the fatty acid which govern the physicochemical properties are the chain length and the position and number of cis-double bonds. All of the major unsaturated w - 6 and w - 3 fatty acids are considered to be essential in that a dietary source is required [ 11. Therefore a great deal of effort has been directed towards understanding the relationship between these fatty acid properties and the physicochemical environment and in turn its effect o n the protein functioning. The primary function of fatty acyl unsaturation is to provide a liquid-crystalline or fluid lipid bilayer phase which will allow the various membrane proteins t o function optimally. An unresolved question is the nature of the control of membrane protein functioning exerted at the level of fatty acyl unsaturation. One direct functional role is of course t o provide the precursors of eicosanoids. These aspects have been extensively reviewed elsewhere and will not be dealt with here (see the other papers in this Colloquium).The release of fatty acids by phospholipase A, will also create altered localizcd physical properties which will differ according to the fatty acid type. In this article the major issue is the relationship beween essential fatty acids and membrane physical properties (for other reviews, see 12-51). Membrane proteins are surrounded by the fatty acyl constituents of membrane phospholipids. To what extent is the function of the protein affected by the nature of the fatty acid in terms of its chain length and unsaturation? This appears to vary considerably from protein to protein. For example, there is strong evidence that Ca?’-ATPase activity is affected more by chain length and is insensitive to the degree of unsaturation [6-8). By contrast, Na’,K+-ATPase does appear to be sensitive to unsaturation 19-1 I]. An important consideration is that just because the reconstituted enzyme activity in question is supported equally well by any crystalline phase phospholipid bilayer, it does not necessarily follow that the enzyme is not subject to more subtle modulation by changes in unsaturation in the natural membrane. In addition, sensitivity of the enzyme to such changes may be lost in a reconstituted enzyme. In general, because these types of questions require complex reconstitution procedures the role of unsaturation has not been examined in many systems. For example, while transport processes examined in intact cells or membrane preparations appear to be very sensitive to modified unsaturation, as modified by dietary or cell-culture means (reviewed in [ 12]), little is known of the response o f particular channel proteins. The fatty acid composition of cell membranes is highly susceptible to dietary manipulation. However, it has become apparent that this manipulation can only occur within very specific limits; for example, an increase in 2 2 : 6 , w 3 at the expense of 20:4,w6 [8,131. This leads to the question of how membrane function may be directly altered by the modified fatty acid composition affecting the physicochemical environment of the membrane. Abbreviations used: T,, gel-liquid-crystalline phase transition temperature; DPH, diphenyl-hexatriene. There are a number of diverse types o f physical properties which can be ascribed to a cell membrane and which are subject to modification by alterations in the level o f unsaturation. In addition, the membrane can be subdivided into at least three distinct areas: the phospholipid head group region, the central hydrocarbon chain region and the region adjacent to membrane proteins. The major physicochemical property of membranes and the most widely studied is known as ‘membrane fluidity’ [ 14). The term membrane fluidity is often misunderstood. The reason why investigation of membrane fluidity is so popular is that it appears to be relatively simple to measure, and can apparently be dealt with as a single physical ‘parameter’. I t is o f course not surprising that such a complex dynamic structure as a cell membrane can only be inadequately described by a single physical parameter. First, it ignores the two basic motional parameters of membranes which can be described as the rate and order. The order relates to the packing of the fatty acid chains which below the gel-liquid-crystalline phase transition temperature ( T,) is highly ordered (all-trans configuration), whereas above 7, the phospholipid fatty acyl chains will contain a number of gauche rotomers that loosen the fatty acid packing and cause a more disordered structure, which is the situation in most mammalian membranes. Thc degree of order and disorder can be obtained from various types of spectroscopic measurements and a parameter relating to the extent of angular motion described by the fatty acid chain segment obtained, i.e. its degree of orientational constraint. How fast the fatty acyl chain describes the angular motion gives the rate of motion. This rate of motion refers (with respect t o ?H-n.m.r., e.s.r. and fluorescence anisotropy measurements) t o rotational motion. Another rate term refers to the lateral motion for which different physical techniques are used 1141. The term membrane fluidity is used in general sense t o cover the rate and order of rotational motion. Probably membrane fluidity should refer only t o the rate of motion; however, the term has taken o n wide usage as a semi-empirical term. In general, the parameters it refers t o are the steady-state fluorescence anisotropy of membrane fluorophore probes rather than the time-resolved fluorescence components o f rate and order [ 141. In this article wc use membrane fluidity only in a general way to cover both the rate and range o f motion as embodied in the steady-state fluorescence anisotropy parameter as commonly measured with the bilayer fluorophorc probe diphenyl-hexatricne (DPH). Another major disadvantage of the use of the term membrane fluidity is that it is by definition a bulk o r average tcrm which applies to the whole membrane in question. This has been an attraction in sim ler organisms and the theory o f homoeoviscous adaptation YlS I has been invoked to describe the maintenance o f membrane fluidity at different growth temperature by an altered lcvel of unsaturation in the phospholipids. However, this rather elegant system does not appear t o translate very well t o more complex mammalian systems, although the basic philosophy behind the idea has influenced the field for a number o f years. Importantly, it does not allow for distinct areas o r regions of differing physical properties t o exist. Such areas have been proposed in the past [ 161 and their attraction is that they allow a membrane to respond t o differing compositional stress from diet or other means by tailoring the properties of specific regions according t o their needs and of buffering sensitive regions from larger changes. Although this approach has obvious attractions there is a lack o f convincing evidence. There are a number of approaches t o the study o f the effect of differing unsaturation on membrane properties. One 780 is to use dietary or cell culture manipulation methods. Dietary methods have been widely used since the results may be o f more immediate direct significance, but again can only be used to obtain modifications within certain limitations. With cell culture thc limitations are less and to answer specific questions the cells can often be forced to incorporate higher levels of a specific test fatty acid than would be possible by dietary means. The third approach is to study model or reconstituted systems where the components of interest can be isolated and a much simplified system can be used consisting only o f the components of interest. The advantage of the latter approach is that conditions can be much more precisely set to test various aspects. It is also possible to isolate particular membrane protein components and to examine these with a precisely defined reconstituted system protein. Since thc extent of modification of the membrane fatty acid composition which the cell will allow is limited, it is not surprising that the physical properties, in terms of bulk or average membrane fluidity parameters, can also only change by small amounts. Thus it seems reasonable to conclude that the reason that the cell will not allow the proportion of saturated fatty acids to change appreciably is because the membrane fluidity would change in an undesirable manner. The same applies to the incorporation of unsaturated fatty acids such as 18:l,w6, 18:2,w6, 18:3,w6, 20:4,w6 or of 2 0 : S , w 3 and 22:6,w3. Faced with an apparently overwhelming dietary or cell-culture challenge of large amounts of these fatty acids, the cell responds by incorporating the fatty acid within fairly modest specified levels and compensating accordingly by reducing the fatty acid which it most nearly resembles. Thus, for example, for a dietary elevation of the highly unsaturated 2 0 : S , w 3 , 22:5,w3 and 22:6,w3, as found in marine-oil-based food products, the 20:4,w6 will decrease accordingly (e.g. [ 81). Of course, although this might maintain the physicochemical equilibrium, it has the potential of changing the type o f eicosanoid formed, allowing other biological effects to occur. One major question which is unresolved is the nature o f the compensation mechanism which appears t o allow sensing o f the membrane physical properties in some form that can be recognized by the cell membrane fatty acyl desaturase-elongase modification system (reviewed in [ 1 71j. We would propose that whatever the nature o f the system for sensing the membrane physical properties in the cell membrane, changes to the membrane fatty acid composition which result in significant overall bulk changes t o the membrane physical properties cannot occur, a process that may be termed a passive type of ’homoeoviscous adaptation’ [ 81. In order t o address the question o f the effect o f fatty acids o n membrane physical properties in localized areas such as domains o r adjacent to proteins, it is important to understand how each typc of unsaturated phospholipid component behaves o n an individual basis. Using this type of approach useful basic information on the behaviour of unsaturated fatty acyl constituents in membranes can be determined. First, with respect to the 7;. it has been established by Keough and co-workers [ 18, 191 that while the first and second cis-double bonds decrease the Tc, further additions into the sn-2 chain o f a phospholipid eventually reverse the effect with further double bonds actually increasing T,. The extreme o f this is 16 : 0 / 2 2:6-phosphatidylcholine where T, is almost the same as that of 16 :O/ I8 : I-phosphatidylcholine [20-221. Also, after the first double bond in a phospholipid, further double bonds have a much diminished effect compared to the first 1241. With the 2 2 : 6 chain it is probably the 16:O sn-1 chain which is actually undergoing the transition due to the increasing stiffness introduced by the inflexible carbon-carbon double bonds and also the helical configuration of the 2 2 : 6 chain ( [ 2 ,21, 251 and see reviews dealing with 2 2 : 6 126, 271). How this chain behaves at the BIOCHEMICAL SOCIETY TRANSACTIONS protein-lipid interface compared with less unsaturated chains is currently a topic of investigation. In addition to the order and rate of acyl chain motion there are other physicochemical properties worthy of investigation. For example, the fluorescence lifetime of a membrane probe such as DPH is highly dependent on its immediate environment or ‘solvent cage’ experienced while in the excited state. By analysing the fluorescence decay process as a distribution of decay rates, the degree of environmental heterogeneity experienced by the fluorophore can be ascertained [28]. This will vary according t o the depth in the bilayer, due to differing degrees of water penetration 128, 291, and this is increased for the more unsaturated fatty acids (C. Ho, B. W. Williams & C. D. Stubbs, unpublished work). A heterogeneity of decay rates is also caused by membrane proteins, probably due to a combination of the hydrophobic amino acid side chains and the adjacent fatty acyl chains [ 3 11. In this case the role of unsaturation remains to be determined. However, due to the potential of this region in influencing protein conformation and function this should be a fruitful area of future investigation. The financial support of PHS grants A A 0 8 0 2 2 and 072 IS and a grant from the Alcoholic Beverage Medical Research Foundation are gratefully acknowledged. I. Vergroesen, A . J . & Crawford, M. (d.) ( I YYO) The Hob, oj’l.ii/.s in Human Nrt/ri/iori Academic Press, London and New York 2. Stubbs, C. D. & Smith, A . D.( I Y84) Hiochim. Hiophys. Acw 779.89-137 3. Spector, A . A . & York, M. A . ( 1 Y 8 S ) J. Lipid Hes. 26, 1 0 I 5- I 035 4. McMurchie, E. J . ( I Y88) in Physiologicd Kegiilciriorr o/’ Mcvnhrcinr Fluidity, pp. I XY-237.Alan Liss. New York 5. Quinn, P. J., JOO, F.& Vigh, L. ( I YXY) /'rag. Hiophys. M o l . I1iol. 53.7 1-1 03 6. East, J . M., Jones, 0.T., Sirnmonds. A . C. & Lee, A . G . (10x4) J . Hiol. (’hem. 259.8070-807I 7. Gould, G.W., McWhirter, J . M., East. J . M. and Lee, A . G . ( I Y87)Biochem. J. 245.75 1-755 8. Stuhbs, C.D.& Kisielewski, A . ( 1090) />Ipil/.s in the press 9. Bruni, A,. van Dijk, P. W. M. & de Gier, J . ( 1075)Hiochinr. Riophys. AC/U406.3 15-328 10. Brivio-Haughland. K. P., Louis. S. L.. Musch, K., Waldcck, N . & Williams, M. A . ( I Y76)Hiochim. l1iophy.s. Acw 433. I SO- 163 I I . Galo, M.G., Unates. L. €5. & Farias. K. N. ( I Y8 I ) J . Hiol. (’hem. 256.71 13-71 I4 12. Spector, A . A,, Mathur. S. N.. Kaducc. I., L. & Hyman. 13. -1. ( I Y 8 1 ) I’rog. LipidKes. 10,56-67 13. Conroy, D. C..Stubbs, C. D., Belin, J.. Pryor. C . L. & Smith. A . D. ( 1986) Biochim. Hiophys. A m 86 1,457-462 14. Stubbs, C.D.( 19x3) I:‘ssriys Biochcwi. 19.I - 3 Y IS. Sinensky, M. (1974)I’roc. N d . Accicl. S c i . U.S.A. 71.522-525 16. Karnovsky, M. J.. Kleinfeld, A . M.. Hoover, K. L. & Klausner. R. D. ( I 982) J . C M mi. 94,I -6 17. Quinn, P. J. ( 198 I ) Prog Hiophy. Mol. Hiol. 38. I - I04 I 8. Keough, K. M. W.. Giffin. B. & Kariel. N. ( I YX7)H i o c h i n i . /1iophy.~.AC/O902.I - I0 19. Keough, K. M. W. & Kariel, N. ( 1987)Hiochini. Hiophys. Acrci 902,II-lX 20. DKKSK, A . J., Dratz, E. A,, Dahlquist, F. W. & Paddy, M. K. ( I98 I ) Hiochemi.s/qj 20.6420-6427 21. Stubbs, C. D., Pryor, C . L., Nie, Y., Taraschi. 1’.F.. Ellingson, J . & Mendelsohn, R. ( 1986) Hiophys. J. 49.3 13 22. Stubbs, C. D. ( 1089) C’O/~OC/. INSEHM 195. 125- I34 23. Reference deleted 24. Stubbs, C. D.. Kouyama, T.. Kinosita. K.. Jr. & Ikegami. A . ( I YX I ) Hiochrmisrr?/20,4257-4262 25. Applegate. K. R. & Glomset. J . A . ( 1 9 8 6 ) J. I i p i c l Hcs. 27, 658-680 26. Salem, N., Kim, H.-Y. & Yergey, J . A . ( I Y86) in Hralrh EJpc~so j ’ I’olyiirisciritrrtred F(i/rj, Acids iri .Secijbods (Simopoulos. A . P.. Kefer. R. R. bi Martin. R. E.. (eds.). pp. 263-3 17. Academic Press. London and New York 78 1 FATTY ACID METABOLISM 27. Dratz. E. A. & Deese, A. J. ( 1986) in Health Eflects of I’olyctn.sutctmted /+city Acids in Secrjbods (Simopoulos. A. P.. Kefer. R. R. & Martin, R. E.. eds.). pp. 263-317, Academic Press, London and New York 28. Williams. B. W. & Stubbs, C. D. (1988) Biochemistry 27, 7994-7999 29. Stubbs, C . D., Williams, B. W. & Ho, C. ( 1990) I’roc. S I ’ I E 30. Reference deleted 3 1. Willliams, B. W.. Scotto. A. W. & Stubbs. C. D. ( 1990) Hiochemistry29,3248-3255 Received 25 April 1990 1204,448-455 Structural and enzymological properties of cellular phospholipases A, HENK VAN DEN BOSCH.* ANTON J. AARSMAN,* RON H. N. VAN SCHAIK? CASPER G. SCHALKWIJK,* FRED W. NEIJS* and AUGUESTE STURKt * Ccritrefor Riometnbranes arid Lipid Enzymology, Universiry of Utrecht, Transitoriiim 3, Padiraluun 8,3.584 CH Utrecht, 71ie Netherlarids. and t Department of Hematology, University of‘Atnster(lam, Academic Medical Center, Meibergdreef 9, I105 AZ Atristerdam. The Netherlands Introdirctiori Phospholipases A,, which catalyse the hydrolysis of acyl cstcr bonds at the sn-2-position of naturally occurring phosphoglycerides, occur widely in nature. Pancreatic juice and snake venoms are rich sources and detailed information on the structure and catalytic mechanism of these enzymes is available [ 11. The enzymes are also found in minute quantities in almost any mammalian cell, often associated with more than one subcellular organelle, at least in vitro after cell disruption [2]. A long-standing question has been what the relationship in structural properties is between the extracellular and cellular enzymes on one hand and between thosc in the different subcellular organelles on the other hand. From the point of view o f cell biology there is a general interest in the regulation of cellular phospholipases A, because the uncontrolled action of the membrane-associated enzymes might easily destroy biomembrane function and compartmentalization in eukaryotic cells. The enzymes have also received much attention because they are implicated in the release of arachidonate and 1- 0-alkyl-2-hydroxy-snglycero-3-phosphocholine (lyso-platelet-activating factor, lyso-PAF ), i.e. precursors for bioactive lipids 13, 41. Whether these precursors are formed by specific phospholipases A? that exhibit specificities for either the polar headgroup, the acyl-chain at the sn-2-position or the type of linkage at the sri-1-position, i.e. an ester or an ether linkage, remains a rather open question at present. This is largely the result of two commonly encountered problems. First, cellular phospholipases A? are extremely low-abundancy proteins and only few of them have been obtained in sufficient amounts and purity for detailed substrate specificity studies. Secondly, the enzymes act at interfaces formed by the waterinsoluble substrates so that the physico-chemical factors that govern substrate organization have a profound effect on enzymic activity, as will be illustrated. It~liierice of substrate organization oti phospholipase A logical as it may be, be reconciled with the well-known phenomenon that membrane-associated phospholipases A, can be assayed with exogenously added substrates? Studies on the substrate selectivity o f the enzyme provided a clue to this problem. The membrane-associated enzyme showed a 2- to 3-fold preference for phosphatidylethanolaminc over phosphatidylcholine hydrolysis when acting on endogenous mitochondrial phospholipids (Fig. 1 ). A comparison o f the two substrates, when added exogenously, indicated that the preference for phosphatidylethanolamine hydrolysis became 20- to 30-fold. At first sight one would be inclined t o conclude from this comparison that the enzyme is rather specific for phosphatidylethanolamine. However, the observed selcctivity does not reflect a true enzyme specificity but appears to be governed by physicochemical factors. Phosphatidylcholine forms stable bilayer membranes that do not intcract well with the mitochondrial membrane and, therefore, is poorly degraded, unless a phosphatidylcholine-exchange protein is included in the incubation mixture t o insert the exogenous substrate into the biomembrane having the enzyme [S].Alternatively, proper contact o f enzyme and substrate can be induced by addition o f detergents. In contrast, phosphatidylethanolaminc. especially in the presencc of Ca2+ ions necessary for measurements of phospholipase A2 activity, forms hexagonal structures that become easily associated with the mitochondrial membranes as could be demonstrated by sucrose-gradient centrifugations 15. I. This BIOMEMBRANE 6.uI EXOGENOUS SUBSTRATE PC MEMBRANE ASSOCIATION MODEL MEMBRANE (PE PC = 40160) PLUS ENZYME .,A PE n , RATIO PWPC 20 - 30 READILY . 3-4 uctivitv Rat liver mitochondria contain a peripherally membraneassociated phospholipase A? that acts exclusively on substrates in its own membrane [S].How can this observation, Abbreviations used: lyso-PAF, lyso-platelet activating factor ( 1 O-alkyl-2-hydroxy-s~~-~lycero-3-ph~~sphoch~~line); PAF, plateletactivating factor. Vol. 18 Fig. 1. Actrori of mernbrutie-associated mitochondria1 phospholipase A 2 towards endogenous arid exogerioiis substrutes The large preference for exogenous phosphatidylethanolm i n e (PE) compared with phosphatidylcholine (PC) is explained by its tendency to form hexagonal structures that become easily associated with the biomembrane containing the enzyme.