Abstract
Proteins are polymers, and yet the language used in describing their thermodynamics and kinetics is most often that of small molecules. Using the terminology and mathematical descriptions of small molecules impedes understanding why proteins have evolved to be big in comparison. Many properties of the proteins should be interpreted as polymer behavior, and these arise because of the longer length scale of polymer dimensions. For example, entropic rubber elasticity arises only because of polymer properties, and understanding the separation of entropic and enthalpic contributions shows that the entropic contributions mostly reside within the polymer and enthalpy originates mostly at the site of small-molecule binding. Recognizing the physical chemistry of polymers in descriptions of proteins’ structure and function can add clarity to what might otherwise appear to be confusing or even paradoxical behavior. Two of these paradoxes include, first, highly selective binding that is, nevertheless, weak, and, second, small perturbations of an enzyme that cause large changes in reaction rates. Further, for larger structures such as proteins every thermodynamic measurement depends on the length scale of the structure. One reason is that the larger molecule can control up to thousands of waters resulting in collective movements with kcal sums of single-calorie-per-molecule solvent energy changes. In addition, the nature of covalent polypeptides commonly leads to multiple binding—i.e., multivalency—and the benefits of multivalent binding can be assessed semiquantitatively drawing from understanding the chelate effect in coordination chemistry. Such approaches clarify the origins, inter alia, of many low energies of protein denaturation, which lie in the range of only a few kcal mol−1, and the difficulties in finding the structures of proteins in the multiple substates postulated within complex kinetic schemes. These models involving longer length scales can be used to elucidate why such observed behavior occurs, and can provide insight and clarity where the phenomena modeled employing experimentally inseparable translational, vibrational, and rotational entropy along with charge, dipole moment, hydration, hydrogen bonding, and van der Waals energies together obscure such origins. The short-distance, long distance separation does not include explaining any enzymatic lowering of activation energies due to stabilization of the intermediate(s) along the reaction path. However, well known small-molecule methods that treat electrostatics and bonding can be used to explain the local chemistry that contributes most of the changes in enthalpy and activation enthalpy for the process.
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References
Koshland DE (1958) Application of a theory of enzyme specificity to protein synthesis. Proc Natl Acad Sci USA 44:98–104
Koshland JDE, Neet KE (1968) The catalytic and regulatory properties of enzymes. Ann Rev Biochem 37:359–411
Careri G, Fasella P, Gratton E (1979) Enzyme dynamics: the statistical physics approach. Ann Rev Biophys Bioeng 8:69–97
Britt BM (1997) For enzymes, bigger is better. Biophys Chem 69:63–70
Eisenmesser EZ, Millet O, Labeikovsky W, Korzhnev DM, Wolf-Watz M, Bosco DA, Skalicky JJ, Kay LE, Kern D (2005) Intrinsic dynamics of an enzyme underlies catalysis. Nature 438(3 November):117–121
Henzler-Wildman KA, Lei M, Thai V, Kerns SJ, Karplus M, Dorothee Kern D (2007) A hierarchy of timescales in protein dynamics is linked to enzyme catalysis. Nature 450(6 December):913–918
Kokkinidis M, Glykos NM, Fadouloglou VE (2012) Protein flexibility and enzymatic catalysis. Adv Prot Chem Struct Biol 87:181–218
Hong L, Glass DC, Nickels JD, Perticaroli S, Yi Z, Madhusudan T, O’Neill H, Zhang Q, Sokolov AP, Smith JC (2013) Elastic and conformational softness of a globular protein. Phys Rev Lett 110:028104
Warshel A, Bora RP (2016) Perspective: defining and quantifying the role of dynamics in enzyme catalysis. J Chem Phys 144:180901
Bar-Even A, Milo R, Noor E, Tawfik DS (2015) The moderately efficient enzyme: futile encounters and enzyme floppiness. Biochemistry 54:4969–4977
Glantz-Gashai Y, Meirson T, Samson AO (2016) Normal modes expose active sites in enzymes. PLoS Comput Biol 12:e1005293
Cram DJ, Lein GM, Kaneda T, Helgeson RC, Knobler CB, Maverick E, Trueblood KN (1981) Augmented and diminished spherands and scales of binding. J Am Chem Soc 103(20):6228–6232
Krishtalik LI, Topolev VV (1983) The intraglobular electrostatic field of an enzyme. 1. The primary field created by the polypeptide core, functional groups and ions of the alpha-chymotrypsin molecule. Molekuliarnaia Biologiia 17(5):1034–1041
Reinhoudt DN, Dijkstra PJ (1988) Role of preorganization in host-guest-chemistry. Pure Appl Chem 60(4):477–482
Bruice TC, Benkovic SJ (2000) Chemical basis for enzyme catalysis. Biochemistry 39(21):6267–6274
Rajamani D, Thiel S, Vajda S, Camacho CJ (2004) Anchor residues in protein–protein interactions. Proc Natl Acad Sci USA 101(31):11287–11292
Nienhaus GU (2006) Exploring protein structure and dynamics under denaturing conditions by single-molecule FRET analysis. Macromol Biosci 6:907–922
Wittenberg JB, Isaacs L (2012) Complementarity and preorganization. In: Steed JW, Gale PA (eds) Supramolecular chemistry: from molecules to nanomaterials. https://doi.org/10.1002/9780470661345.smc004/full
Kitov PI, Bundle DR (2003) On the nature of the multivalency effect: a thermodynamic model. J Am Chem Soc 125:16271–16284
Badjić JD, Nelson A, Cantrill SJ, Turnbull WB, Stoddart JF (2005) Multivalency and cooperativity in supramolecular chemistry. Acc Chem Res 38:723–732
Sun H, Hunter CA, Navarro C, Turega S (2013) Relationship between chemical structure and supramolecular effective molarity for formation of intramolecular H-bonds. J Am Chem Soc 135:13129–13141
Rand RP (1981) Interacting phospholipid bilayers: measured forces and induced structural changes. Ann Rev Biophys Bioeng 10:277–314
Pabst G, Rappolt M, Amenitsch H, Laggner P (2000) Structural information from multilamellar liposomes at full hydration: full q-range fitting with high quality x-ray data. Phys Rev E 62(3):4000–4009
Filfil R, Chalikian TV (2003) The thermodynamics of protein–protein recognition as characterized by a combination of volumetric and calorimetric techniques: the binding of turkey ovomucoid third domain to α-chymotrypsin-chymotrypsin. J Mol Biol 326:1271–12288
Fisette O, Päslack C, Barnes R, Isas JM, Langen R, Heyden M, Han S, Schäfer LV (2016) Hydration dynamics of a peripheral membrane protein. J Am Chem Soc 138:11526–11535
Rubinson KA, Meuse CW (2013) Deep hydration: poly(ethylene glycol) Mw 2000-8000 Da probed by vibrational spectrometry and small-angle neutron scattering and assignment of ΔG° to individual water layers. Polymer 54:709–723
Cheng C-Y, Varkey J, Ambroso MR, Langen R, Han S (2013) Hydration dynamics as an intrinsic ruler for refining protein structure at lipid membrane interfaces. Proc Natl Acad Sci USA 110:16838–16843
Xu Y, Havenith M (2015) Perspective: watching low-frequency vibrations of water in biomolecular recognition by THz spectroscopy. J Chem Phys 143:170901
Munro D (1977) Misunderstandings over the chelate effect. Chem Britain 13(3):100–105
Cotton FA, Harris FE (1956) The thermodynamics of chelate formation. II. A Monte Carlo study of the distributions of configurations in short chains. J Phys Chem 60(10):1451–1454
Carter MJ, Beattie JK (1970) The kinetic chelate effect. Chelation of ethylenediamine on platinum(II). Inorg Chem 9(5):1233–1238
Wolfenden R, Snider MJ (2001) The depth of chemical time and the power of enzymes as catalysts. Acc Chem Res 34(12):938–945
Naganathan AN (2019) Modulation of allosteric coupling by mutations: from protein dynamics and packing to altered native ensembles and function. Curr Opin Struct Biol 54:1–9
Vogt AD, Di Cera E (2012) Conformational selection or induced fit? A critical appraisal of the kinetic mechanism. Biochemistry 51:5894–5902
Vogt AD, Di Cera E (2013) Conformational selection is a dominant mechanism of ligand binding. Biochemistry 52:5723–5729
Gianni S, Dogan J, Jemth P (2014) Distinguishing induced fit from conformational selection. Biophys Chem 189:33–39
Cabbiness DK, Margerum DW (1970) Effect of macrocyclic structures on the rate of formation and dissociation of copper(II) complexes. J Am Chem Soc 92(7):2131–2133
Lightstone FC, Bruice TC (1996) Ground state conformations and entropic and enthalpic factors in the efficiency of intramolecular and enzymatic reactions. 1. Cyclic anhydride formation by substituted glutarates, succinate, and 3,6-endoxo-D4-tetrahydrophthalate monophenyl esters. J Am Chem Soc 118:2595–2605
Rosker MJ, Dantus M, Zewail AH (1988) Femtosecond clocking of the chemical bond. Science 241:1200–1202
Jönsson P-G (1971) Hydrogen bond studies. XLIV. neutron diffraetion study of acetie acid. Acta Cryst B27:893–898
Robl C, Hentschel S, McIntyer GJ (1992) Hydrogen bonding in Be[C2(COO)2]·4H2O–a neutron diffraction study at 15 K. J Solid State Chem 96:318–323
Elles CG, Crim FF (2006) Connecting chemical dynamics in gases and liquids. Annu Rev Phys Chem 57:273–302
Goryainov SV (2012) A model of phase transitions in double-well Morse potential: application to hydrogen bond. Phys B 407:4233–4237
Ishikita H, Saito K (2016) Proton transfer reactions and hydrogen-bond networks in protein environments. J R Soc Interface 11:20130518
Blinc R, Hadži D, Novak A (1960) The relation between the bridge length of short hydrogen bonds, the potential curve, and the hydroxyl stretching frequency. Beri Bunsenge Phys Chem 64(5):567–571
Emsley J (1980) Very strong hydrogen bonding. Chem Soc Rev 1:91–124
Batsanov SS (2001) Van der Waals Radii of Elements. Inorg Mater 37(9):871–885
Mantina M, Chamberlin AC, Valero R, Cramer CJ, Truhlar DG (2009) Consistent van der Waals Radii for the Whole Main Group. J Phys Chem A 113:5806–5812
Menger FM (1983) Directionality of organic reactions in solution. Tetrahedron 39(7):1013–1040
Menger FM (1985) On the source of intramolecular and enzymatic reactivity. Acc Chem Resh 18:128–132
Karaman R (2010) A general equation correlating intramolecular rates with ‘attack’ parameters: distance and angle. Tetrahedron Lett 51:5185–5190
Rini M, Kummrow A, Dreyer J, Nibbering ETJ, Elsaesser T (2002) Femtosecond mid-infrared spectroscopy of condensed phase hydrogen-bonded systems as a probe of structural dynamics. Faraday Discuss 122:27–40
Menger FM, Chow JF, Kaiserman H, Vasquez PC (1983) Directionality of proton transfer in solution. three systems of known angularity. J Am Chem Soc 105:4996–5002
Robinson RA, Stokes RH (1959) Electrolyte solutions, 2nd edn. Butterworths, Appendices 11.1 & 11.2, London
Rubinson KA (1984) Regularity in protonation and rate constants and the structures in solution of reactants containing a benzene ring. J Phys Chem 88:148–156
Rühmann EH, Rupp M, Betz M, Heine A, Klebe G (2016) Boosting affinity by correct ligand preorganization for the S2 pocket of thrombin: a study by isothermal titration calorimetry, molecular dynamics, and high-resolution crystal structures. ChemMedChem 11:309–319
Urry DW, Hugel T, Seitz M, Gaub HE, Sheiba L, Dea J, Xu J, Parker T (2002) Elastin: a representative ideal protein elastomer. Philo Trans R Soc Lond B 357:169–184
Bryan PN, Orban J (2010) Proteins that swich folds. Curr Opin Struct Biol 20:482–488
Proter LL, He Y, Chen Y, Orban J, Bryan PN (2015) Subdomain interactions foster the design of two protein pairs with ~ 80% sequence identity but different folds. Biophys J 108:154–162
Wong K-B, Yu H-A, Chan C-H (2012) Energetics of protein folding. In: Egelman EH (ed) Comprehensive biophysics, vol 3. Academic Press, New York, pp 19–33
Dobry A, Fruton JS, Sturtevant JM (1952) Thermodynamics of hydrolysis of peptide bonds. J Biol Chem 195:149–154
Borsook H (1953) Peptide bond formation. Adv Prot Chem 8:127–174
Martin RB (1998) Free energies and equilibria of peptide bond hydrolysis and formation. Biopolymers 45:351–353
Xiong K, Asciutto EK, Madura JD, Asher SA (2009) Salt dependence of an α-helical peptide folding energy landscapes. Biochem 48:10818–10826
Bryson JW, Betz SF, Lu HS, Suich DJ, Zhou HX, O’Neil KT, DeGrado WF (1995) Protein design: a hierarchic approach. Science 270:935–941
Pace CN, Scholtz JM (1998) A helix propensity scale based on experimental studies of peptides and proteins. Biophys J 75:422–427
Scholtz JM, Qian H, Robbins VH, Baldwin RL (1993) The energetics of ion-pair and hydrogen-bonding interactions in a helical peptide. Biochemistry 32:9668–9676
Muñoz V, Serrano L (1995) Elucidating the folding problem of helical peptides using empirical parameters. II. Helix macrodipole effects and rational modification of the helical content of natural peptides. J Mol Biol 245:275–296
Yang J, Spek EJ, Gong Y, Zhou H, Kallenbach NR (1997) The role of context on α-helix stabilization: host-guest analysis in a mixed background peptide model. Prot Sci 6:1264–1272
Kim C, Berg JM (1993) Thermodynamic β-sheet propensities measured using a zinc-finger host peptide. Nature 362:267–270
Warshel A, Sharma PK, Kato M, Xiang Y, Liu H, Olsson MHM (2006) Electrostatic basis for enzyme catalysis. Chem Rev 106(8):3210–3235
Kamerlin SCL, Warshel A (2009) At the dawn of the 21st century: is dynamics the missing link for understanding enzyme catalysis? Proteins 78:1339–1375
Flory PJ (1953, Chap. XI) Principles of polymer chemistry. Cornell University Press, Ithaca
Rubinson KA (1986) Closed channel-open channel equilibrium of the sodium channel of nerve: simple models of macromolecular equilibria. Biophys Chem 25:57–72
Flory PJ (1988, Chap. VIII) Statistical mechanics of chain molecules. Hanser, Munich
Rajasekaran N, Sekhar A, Naganathan AN (2017) A Universal pattern in the percolation and dissipation of protein structural perturbations. J Phys Chem Lett 8:4779–4784
Fischer S, Smith JC, Verma CS (2001) Dissecting the vibrational entropy change on protein/ligand binding: burial of a water molecule in bovine pancreatic trypsin inhibitor. J Phys Chem B 105:8050–8055
Nicolaï A, Delarue P, Senet P (2015) Intrinsic localized modes in proteins. Sci Rep 5:18128
Kalescky R, Zhou H, Liu J, Tao P (2016) Rigid residue scan simulations systematically reveal residue entropic roles in protein allostery. PLoS Comput Biol 12(4):e1004893
Smith JC (1991) Protein dynamics: comparison of simulations with inelastic neutron scattering experiments. Q Rev Biophys 24(3):227–291
Houk KN, Leach AG, Kim SP, Zhang X (2003) Binding affinities of host–guest, protein–ligand, and protein–transition-state complexes. Angew Chem Int Ed Engl 42:4872–4897
Fitter J (2003) A measure of conformational entropy change during thermal protein unfolding using neutron spectroscopy. Biophys J 84:3924–3930
Rubinson KA (1998) The polymer basis of kinetics and equilibria of enzymes: the accessible-volume origin of entropy changes in a class Aβ-lactamase. J Protein Chem 17(8):771–787
Christensen BE, Smidsrød O, Stokke BT (1996) Metastable, partially depolymerized xanthans and rearrangements toward perfectly matched duplex structures. Macromolecules 29:2939–2944
Levitt M (2014) Birth and future of multiscale modeling for macromolecular systems. Angew Chem Int Ed Engl 53:10006–10018
Bailey RT, North AM, Pethrick RA (1981, Ch. 13) Molecular motion in high polymers. Clarendon Press, Oxford
Richards EG (1980) An introduction to physical properties of large molecules in solution. Cambridge University Press, Cambridge
Frey E, Kroy K (2005) Brownian motion: a paradigm of soft matter and biological physics. Ann Phys (Leipzig) 14:20–50
Schulz GE (1992) Induced-fit movements in adenylate kinases. Farad Disc 93:85–93
Berry MB, Meador B, Bilderback T, Liang P, Glaser M, Phillips GN Jr (1994) The closed conformation of a highly fexible protein: the structure of E. coli adenylate kinase with bound AMP and AMPPNP. Proteins Struct Funct Genet 19:183–198
Natarajan K, McShan AC, Jiang J, Kumirov VK, Wang R, Zhao H, Schuck P, Tilahun ME, Boyd LF, Ying J, Bax A, Margulies DH, Sgourakis NG (2017) An allosteric site in the T-cell receptor Cb domain plays a critical signalling role. Nat Commun 8:15260
Jacobson H, Stockmayer WH (1950) Intramolecular reaction in polycondensations. I. The theory of linear systems. J Chem Phys 18:1600–1606
Shoemaker BA, Wang J, Wolynes PG (1997) Structural correlations in protein folding funnels. Proc Natl Acad Sci USA 94:777–782
Rupley JA, Gratton E, Careri G (1983) Water and globular proteins. TIBS 8(1):18–22
Thanki N, Thornton JM, Goodfellow JM (1988) Distributions of water around amino acid residues in proteins. J Mol Biol 202:637–657
Menger FM (1993) Enzyme reactivity from and organic perspective. Acc Chem Res 26:206–212
Krokoszyńska I, Otlewski J (1996) Thermodynamic stability effects of single peptide bond hydrolysis in protein inhibitors of serine proteinases. J Mol Biol 256:793–802
Siebert X, Amzel LM (2004) Loss of translational entropy in molecular associations. Proteins 54(1):104–115
Fenimore PW, Frauenfelder H, McMahon BH, Yound RD (2004) Bulk-solvent and hydration-shell fluctuations, similar to α- and β-fluctuations in glasses, control protein motions and functions. Proc Natl Acad Sci USA 101(40):14408–14413
Ball P (2008) Water as an active constituent in cell biology. Chem Rev 180:74–108
Paciaroni A, Cornicchi E, Marconi M, Orecchini A, Petrillo C, Haertlein M, Moulin M, Sacchetti F (2009) Coupled relaxations at the protein–water interface in the picosecond time scale. J R Soc Interface 6:S635–S640
Biela A, Betz M, Heine A, Klebe G (2012) Water makes the difference: rearrangement of water solvation layer triggers non-additivity of functional group contributions in protein–ligand binding. ChemMedChem 7:1423–1434
Le Caër S, Klein G, Ortiz D, Lima M, Devineau S, Pin S, Brubach J-B, Roy P, Pommeret S, Leibl W, Righini R, Renault JP (2014) The effect of myoglobin crowding on the dynamics of water: an infrared study. Phys Chem Chem Phys 16:22841–22852
Nibali VC, Havenith M (2014) New insights into the role of water in biological function: studying solvated biomolecules using terahertz absorption spectroscopy in conjunction with molecular dynamics simulations. J Am Chem Soc 136:12800–12807
Pace CN, Scholtz JM, Grimsley GR (2014) Forces stabilizing proteins. FEBS Lett 588:2177–2184
Carugo O (2016) When proteins are completely hydrated in crystals. Intl J Biol Macromol 89:137–143
Krimmer SG, Cramer J, Betz M, Fridh V, Karlsson R, Heine A, Klebe G (2016) Rational design of thermodynamic and kinetic binding profiles by optimizing surface water networks coating protein-bound ligands. J Med Chem 59:10530–10548
Aoki K, Shiraki K, Hattori T (2016) Salt effects on the picosecond dynamics of lysozyme hydration water investigated by terahertz time-domain spectroscopy and an insight into the Hofmeister series for protein stability and solubility. Phys Chem Chem Phys 18:15060–15069
Comez L, Paolantoni M, Sassi P, Corezzi S, Morresi A, Fioretto D (2016) Molecular properties of aqueous solutions: a focus on the collective dynamics of hydration water. Soft Matter 12:5501–5514
Bellissent-Funel M-C, Hassanali A, Havenith M, Henchman R, Pohl P, Sterpone F, van der Spoel D, Xu Y, Garcia AE (2016) Water determines the structure and dynamics of proteins. Chem Rev 116:7673–7697
Jha A, Ishii K, Udgaonkar JB, Tahara T, Krishnamoorthy G (2011) Exploration of the correlation between solvation dynamics and internal dynamics of a protein. Biochemistry 50:397–408
Pal SK, Peon J, Zewail AH (2002) Biological water at the protein surface: dynamical solvation probed directly with femtosecond resolution. Proc Natl Acad Sci USA 99(4):1763–1768
Qin Y, Zhang L, Wang L, Zhong D (2017) Observation of the global dynamic collectivity of a hydration shell around apomyoglobin. J Phys Chem Lett 8:1124–1131
Shiraga K, Ogawa Y, Kondo N (2016) Hydrogen bond network of water around protein investigated with terahertz and infrared spectroscopy. Biophys J 111:2629–2641
Ebbinghaus S, Kim SJ, Heyden M, Yu X, Heugen U, Gruebele M, Leitner DM, Havenith M (2007) An extended dynamical hydration shell around proteins. Proc Natl Acad Sci USA 104:20749–20752
Sushko O, Dubrovka R, Donnan RS (2015) Sub-terahertz spectroscopy reveals that proteins influence the properties of water at greater deistances than previously detected. J Chem Phys 142:055101
Ding T, Li R, Zeitler JA, Huber TL, Gladden LF, Middelberg APJ, Falconer RJ (2010) Terahertz and far infrared Spectroscopy of alanine-rich peptides having variable ellipticity. Opt Express 18(26):27431–27444
King JT, Arthur EJ, Brooks CL, Kubarych KJ (2013) Crowding induced collective hydration of biological macromolecules over extended distances. J Am Chem Soc 136:188–194
Glancy P, Beyermann WP (2010) Dielectric properties of fully hydrated nucleotides in the terahertz frequency range. J Chem Phys 132:245102
Heyden M, Bründermann E, Heugen U, Niehues G, Leitner DM, Havenith M (2008) Long-range influence of carbohydrates on the solvation dynamics of watersanswers from terahertz absorption measurements and molecular modeling simulations. J Am Chem Soc 130:5773–5779
Higgins MJ, Polcik M, Fukuma T, Sader JE, Nakayama Y, Jarvis SP (2006) Structured water layers adjacent to biological membranes. Biophys J 91:2532–2542
Grossmann C, Tintinger R, Zhu J, Maurer G (1995) Aqueous two-phase systems of poly(ethylene glycol) and dextran–experimental results and modeling of thermodynamic properties. Fluid Phase Equilib 106:111–138
Basdogan Y, Keith JA (2018) A paramedic treatment for modeling explicitly solvated chemical reaction mechanisms. Chem Sci 9:5341
Pashley RM, Kitchener JA (1979) Surface forces in adsorbed multilayers of water on quartz. J Colloid Interface Sci 71(3):491–500
Soper AK (2007) Joint structure refinement of x-ray and neutron diffraction data on disordered materials: application to liquid water. J Phys 19:335206
J-m Zheng, Chin W-C, Khijniak E, Khijniak E Jr, Pollack GH (2006) Surfaces and interfacial water: evidence that hydrophilic surfaces have long-range impact. Adv Colloid Interface Sci 127:19–27
Urry DW (1997) Physical chemistry of biological free energy transduction as demonstrated by elastic protein-based polymers. J Phys Chem B 101:11007–11028
Grunwald E, Comeford LL (1995) Thermodynamic mechanisms for enthalpy-entropy compensation. In: Gregory RB (ed) Protein-solvent interactions. Marcel Dekker, New York, pp 421–443
Sharp K (2001) Entropy–enthalpy compensation: fact or artifact? Prot Sci 10(3):661–667
Lumry R (2003) Uses of enthalpy–entropy compensation in protein research. Biophys Chem 105:545–557
Mammen M, Choi S-K, Whitesides GM (1998) Polyvalent interactions in biological systems: implications for design and use of multivalent ligands and inhibitors. Angew Chem Int Ed Engl 37:2754–2794
Williams DH, Stephens E, O’Brien DP, Zhou M (2004) Understanding noncovalent interactions: ligand binding energy and catalytic efficiency from ligand-induced reductions in motion within receptors and enzymes. Angew Chem Int Ed Engl 43:6596–6616
Oshovsky GV, Reinhoudt DN, Verboom W (2007) Supramolecular chemistry in water. Angew Chem Int Ed Engl 46:2366–2393
Cram DJ (1986) Preorganization—from solvents to spherands. Angew Chem Int Ed Engl 25(12):1039–1057
Martell AE, Hancock RD, Motekaitis RJ (1994) Factors affecting stabilities of chelate, macrocyclic, and macrobicyclic complexes in solution. Coord Chem Rev 133:39–65
Piguet C (2010) Five thermodynamic describers for addressing serendipity in the self-assembly of polynuclear complexes in solution. Chem Commun 46:6209–6231
DiMaio J, Gibbs B, Munn D, Lefebvre J, Konishi Y (1990) Bifunctional thrombin inhibitors based on the sequence of hirudin45-65. J Biol Chem 265(35):21698–21703
Fersht AR (1997) Nucleation mechanisms in protein folding. Curr Opin Struct Biol 7:3–9
Pappu RV, Srinivasan R, Rose GD (2000) The Flory isolated-pair hypothesis is not valid for polypeptide chains: implications for protein folding. Proc Natl Acad Sci USA 97:12565–12570
Fitzkee NC, Rose GD (2004) Reassessing random-coil statistics in unfolded proteins. Proc Natl Acad Sci USA 101:12497–12502
Kauffman S, Levin S (1987) Towards a general theory of adaptive walks on rugged landscapes. J Theor Biol 128(1):11–45
Figliuzzi M, Jacquier H, Schug A, Tenaillon O, Weigt M (2016) Coevolutionary landscape inference and the context-dependence of mutations in beta-lactamase TEM-1. Mol Biol Evol 33(1):268–280
Hopf TA, Ingraham JB, Poelwijk FJ, Schärfe CPI, Springer M, Sander C, Marks DS (2017) Mutation effects predicted from sequence co-variation. Nat Biotech 35(2):128–135
Izatt RM, Pawlak K, Bradshaw JS, Bruening RL (1991) Thermodynamic and kinetic data for macrocycle interactions with cations and anions. Chem Rev 91(8):1721–2085
Lashley MA, Ivanov AS, Bryantsev VS, Dai S, Hancock RD (2016) Highly preorganized ligand 1,10-phenanthroline-2,9-dicarboxylic acid for the selective recovery of uranium from seawater in the presence of competing vanadium species. Inorg Chem 55:10818–10829
Schneider H-J (2009) Binding mechanisms in supramolecular complexes. Angew Chem Int Ed Engl 48:3924–3977
Page MI, Jencks WP (1971) Entropic contributions to rate accelerations in enzymic and intramolecular reactions and the chelate effect. Proc Natl Acad Sci USA 68:1678–1683
Newberry RW, Raines RT (2016) A prevalent intraresidue hydrogen bond stabilizes proteins. Nat Chem Biol 12(12):1084–1088
Jencks WP (1981) On the attribution and additivity of binding energies. Proc Natl Acad Sci USA 78(7):4046–4050
Cabbiness DK, Margerum DW (1969) Macrocyclic effect on the stability of copper(II) tetramine complexes. J Am Chem Soc 91(23):6540–6541
Sokol LSWL, Ochrymowycz LA, Rorabacher DB (1981) Macrocyclic, ring size, and anion effects as manifested in the equilibrium constants and thermodynamic parameters of copper(II)-cyclic polythia ether complexes. Inorg Chem 20:3189–3195
Mandolini L (1986) Intramolecular reactions of chain molecules. Adv Phys Org Chem 22:1–111
Illuminati G, Mandolini L, Masci B (1977) Ring-closure reactions. 9. Kinetics of ring formation from o-ω-bromoalkoxy phenoxides and o-ω-bromoalkyl phenoxides in the range of 11- to 24-membered rings. A Comparison with related cyclization series. J Am Chem Soc 99(19):6308–6312
Smith GF, Margerum DW (1975) Diminution of the macrocyclic effect for nickel(II) complexes of thioethers in nonaqueous solvents. J C S Chem Commun 807–808
Schwarzenbach G (1952) Der chelateffect. Helv Chim Acta 35(7):2344–2359
Rubinson KA (2014) Small-angle neutron scattering of aqueous SrI2 suggests a mechanism for ion transport in molecular water. J Solut Chem 43:453–464
Evstigneev MP, Lantushenkoa AO, Golovchenkoa IV (2016) Hidden entropic contribution in the thermodynamics of molecular complexation. Phys Chem Chem Phys 18:7617–7626
Faver JC, Benson ML, He X, Roberts BP, Wang B, Marshall MS, Sherrill CD, Merz KMJ (2011) The energy computation paradox and ab initio protein folding. PLoS ONE 6(4):e18868
Rabinowitch E (1937) Collision, co-ordination, diffusion and reaction velocity in condensed systems. Trans Farad Soc 33:1225–1233
Laidler KJ (1987) Chemical kinetics. Harper & Row Publishers, New York
Feller W (1968) An introduction to probability theory and its applications, vol. I, 3rd edn. Wiler, New York, pp 67–97
Owusu-Apenten RK (1995) A three-state heat-denaturation of bovine α-lactalbumin. Food Chem 52:131–133
Wong K-B, Freund SMV, Fersht AR (1996) Cold denaturation of barstar: 1H, 15N and 13C NMR assignment and characterisation of residual structure. J Mol Biol 259:805–818
Shortle D (1996) The denatured state (the other half of the folding equation) and its role in protein stability. FASEB J 10(1):27–34
Zaidi FN, Nath U, Udgaonkar JB (1997) Multiple intermediates and transition states during protein unfolding. Nat Struct Biol 4(12):1016–1024
Zocchi G (1997) Proteins unfold in steps. Proc Natl Acad Sci USA 94:10647–10651
Bowler BE (2007) Thermodynamics of protein denatured states. Mol BioSyst 3:88–99
Jensen MR, Markwick PRL, Meier S, Griesinger C, Zweckstetter M, Grzesiek S, Bernado P, Blackledge M (2009) Quantitative determination of the conformational properties of partially folded and intrinsically disordered proteins using NMR dipolar couplings. Structure 17:1169–1185
Stefanowicz P, Petry-Podgorska I, Kowelewska K, Jaremko L, Jreemko M, Szewczuk Z (2010) Electrospray ionization mass spectrometry as a method for studying the high-pressure denaturation of proteins. Biosci Rep 30:91–99
Receveur-Bréchot V, Durand D (2012) How random are intrinsically disordered proteins? A small angle scattering perspective. Curr Prot Peptide Sci 13:55–75
Lumry R, Biltonen R (1966) Validity of the “two-state” hypothesis for conformational transitions of proteins. Biopolymers 4:917–944
Amor BRC, Schaub MT, Yaliraki SN, Barahona M (2016) Prediction of allosteric sites and mediating interactions through bond-to-bond propensities. Nat Commun 7:12477
Rajasekaran N, Suresh S, Gopi S, Raman K, Naganathan AN (2017) A general mechanism for the propagation of mutational effects in proteins. Biochemistry 56:294–305
Ayaz P, Munyoki S, Geyer EA, Piedra1 F-A, Vu1 ES, Bromberg R, Otwinowski Z, Grishin NV, Brautigam CA, Rice LM (2014) A tethered delivery mechanism explains the catalytic action of a microtubule polymerase. eLife 3:03069
Hamilton CL, Niemann C, Hammond GS (1966) A quantitative analysis of the binding of N-acyl derivatives of α-aminoamides by α-chymotrypsin. Proc Natl Acad Sci USA 55(3):664–669
Niemann C (1964) Alpha-chymotrypsin and the nature of enzyme catalysis. Science 143:1287–1296
Vitagliano L, Merlino A, Zagari A, Mazzarella L (2000) Productive and nonproductive binding to ribonuclease A: X-ray structure of two complexes with uridylyl(2′,5′)guanosine. Protein Sci 9:1217–1225
Freire E (1999) The propagation of binding interactions to remote sites in proteins: analysis of the binding of the monoclonal antibody D1.3 to lysozyme. Proc Natl Acad Sci USA 96:10118–10122
Pan H, Lee JC, Hilser VJ (2000) Binding sites in Escherichia coli dihydrofolate reductase communicate by modulating the conformational ensemble. Proc Natl Acad Sci USA 97(22):12020–20125
Gunasekaran K, Ma B, Nussinov R (2004) Is allostery an intrinsic property of all dynamic proteins? Proteins 57:433–443
Long D, Brüschweiler R (2011) Atomistic kinetic model for population shift and allostery in biomolecules. J Am Chem Soc 133:18999–19005
Wei G, Xi W, Nussinov R, Ma B (2016) Protein ensembles: how does nature harness thermodynamic fluctuations for life? The diverse functional roles of conformational ensembles in the cell. Chem Rev 116:6516–6551
Dagliyan O, Tarnawski M, Chu P-H, Shirvanyants D, Schlichting I, Dokholyan NV, Hahn KM (2016) Engineering extrinsic disorder to control protein activity in living cells. Science 354(6318):1441–1444
Segel IH (1993) Enzyme kinetics. Wiley, New York
Neher E, Sakmann B (1976) Single-channel currents recorded from membrane of denervated frog muscle fibres. Nature 760(April 29):799–802
Keller BU, Hartshorne RP, Talvenheimo JA, Catterall WA, Montal M (1986) Sodium channels in planar lipid bilayers: channel gating kinetics of purified sodium channels modified by batrachotoxin. J Gen Physiol 88:1–23
Rubinson KA (1992) Steady-state kinetics of solitary bachtrachotoxin-treated sodium channels. Kinetics on a bounded continuum of polymer conformations. Biophys J 61:463–479
Eggeling C, Fries JR, Brand L, Günther R, Seidel CAM (1998) Monitoring conformational dynamics of a single molecule by selective fluorescence spectroscopy. Proc Natl Acad Sci USA 95:1556–1561
Xie XS, Lu HP (1999) Single-molecule enzymology. J Biol Chem 274:15967–15970
English BP, Min W, van Oijen AM, Lee KT, Luo G, Sun H, Cherayil BJ, Kou SC, Xie S (2006) Ever-fluctuating single enzyme molecules: Michaelis-Menten equation revisited. Nat Chem Biol 2(2):87–94
Volkman BF, Lipson D, Wemmer DE, Kern D (2001) Two-state allosteric behavior in a single-domain signaling protein. Science 291(23 March):2429–2433
Lisi GP, Loria JP (2016) Solution NMR spectroscopy for the study of enzyme allostery. Chem Rev 116:6323–6369
Otrusinová O, Demo G, Padrta P, Jaseňáková Z, Pekárová B, Gelová Z, Szmitkowska A, Kadeřávek P, Jansen S, Zachrdla M, Klumpler T, Marek J, Hritz J, Janda L, Iwaï H, Wimmerová M, Hejátko J, Źídek L (2017) Conformational dynamics are a key factor in signaling mediated by the receiver domain of a sensor histidine kinase from Arabidopsis thaliana. J Biol Chem 292(42):17525–17540
Koshland DE (1994) The key-lock theory and the induced fit theory. Angew Chem Int Ed Eng 33:2375–2378
Warshel A (1978) Energetics of enzyme catalysis. Proc Natl Acad Sci USA 75(11):5250–5254
Liu H, Warshel A (2007) The catalytic effect of dihydrofolate reductase and its mutants is determined by reorganization energies. Biochemistry 46:601–6025
Fried SD, Bagchi S, Goxer SG (2014) Extreme electric fields power catalysis in the active site of ketosteroid isomerase. Science 346(6216):1510–1514
Fried SD, Boxer SG (2017) Electric fields and enzyme catalysis. Annu Rev Biochem 86:387–415
Morgenstern A, Jaszai M, Eberhart ME, Alexandrova AN (2017) Quantified electrostatic preorganization in enzymes using the geometry of the electron charge density. Chem Sci 8:5010–5018
Blomberg MRA, Siegbahn PEM (2010) Quantum chemistry as a tool in bioenergetics. Biochim Biophys Acta 1797:129–142
Kim KH, Kim JG, Nozawa S, Sato T, Oang KY, Kim TW, Jo HKJ, Park S, Song C, Sato T, Ogawa K, Togashi T, Tono K, Yabashi M, Ishikawa T, Kim J, Ryoo R, Kim J, Ihee H, S-i Adachi (2015) Direct observation of bond formation in solution with femtosecond X-ray scattering. Nature 518(7539):385–389
Shiró G, Natali F, Cupane A (2012) Physical origin of anharmonic dynamics in proteins: new insights from resolution-dependent neutron scattering on homomeric polypeptides. Phys Rev Lett 109:128102
Morresi A, Mariani L, Distefano MR, Giorgini MG (1995) Vibrational relaxation processes in isotropic molecular liquids. A critical comparison. J Raman Spec 26:179–216
Lambert FL (2002) Entropy is simple, qualitatively. J Chem Educ 79(10):1241–1246
Takeuchi H, Allen G, Suzuki S, Dianoux AJ (1980) Low frequency vibraions in solid n-butane and n-hexane by incoherent inelastic neutron scattering. Chem Phys 51:197–203
Giraud G, Karolin J, Wynne K (2003) Low-frequency modes of peptides and globular proteins in solution observed by ultrafast OHD-RIKES spectroscopy. Biophys J 85:1903–1913
Levitt M, Sander C, Stern PS (1985) Protein normal-mode dynamics: trypsin inhibitor, crambin, ribonuclease and lysozyme. J Mol Biol 181:423–447
Silverstein RM, Bassler GC, Morrill TC (1974) Spectrometric identification of organic compounds, 3rd edn. Wiley, Ch, p 3
Schachtschneider JH, Snyder RG (1963) Vibrational analysis of the n-paraffins-II. Normal co-ordinate calculations. Spectrochim Acta 19:117–168, esp. Table 114
Scott DW, El. Sabban MZ (1969) A valence force field for aliphatic sulfur compounds: alkanethiols and thioalkanes. J Mol Spectrosc 30:317–337, esp. Table II
Herzberg G (1950) Spectra of diatomic molecules, 2nd edn. Van Nostrand, Princeton, NJ, p 91
Ginn SGW, Wood JL (1967) The intermolecular stretching vibration of some hydrogen-bonded complexes. Spectrochim Acta 23A:611–625
Miyazawa T, Pitzer KS (1959) low frequency vibrations, polarizability and entropy of carboxylic acid dimers. J Am Chem Soc 81:74–79
Matsushima N, Hikichi K, Tsutsumi A, Kaneko M (1976) X-ray scattering of synthetic poly(α-amino acid)s in the solid state. III. Temperature dependence of the 1.5 Å-meridional reflection of the α-helix. Polymer J 8:88–95
Bustamante C, Smith SB, Liphardt J, Smith D (2000) Single-molecule studies of DNA mechanics. Curr Opin Struct Biol 10:279–285
Efimova YM, Haemers S, Wierczinski B, Norde W, van Well AA (2006) Stability of globular proteins in H2O and D2O. Biopolymers 85(3):264–273
Lassalle MW, Yamada H, Akasaka K (2000) The pressure-temperature free energy-landscape of staphylococcal nuclease monitored by 1H NMR. J Mol Biol 298:293–302
Klotz IM (1996) Equilibrium constants and free energies in unfolding of proteins in urea solutions. Proc Natl Acad Sci USA 93:14411–14415
Ahmad F, Bigelow CC (1982) Estimation of the free energy of stabilization of ribonuclease A, lysozyme, α-lactalbumin, and myoglobin. J Biol Chem 257(21):12935–12938
Nojima H, Ikai A, Oshima T, Noda H (1977) Reversible thermal unfolding of thermostable phosphoglycerate kinase. Thermostability associated with mean zero enthalpy change. J Mol Biol 116:429–442
Privalov PL, Khechinashvili NN (1974) A thermodynamic approach to the problem of stabilization of globular protein structure: a calorimetric study. J Mol Biol 86:665–684
Beadle BM, McGovern SL, Patera A, Shoichet BK (1999) Functional analyses of AmpC β-lactamase through differential stability. Prot Sci 8:1816–1824
Acknowledgements
I am pleased to thank the following colleagues for reading and commenting on the typescript: Lawrence Prochaska, Gerald Alter, David Hoogerheide, Joseph Hubbard, Lawrence Berliner, Susana Teixeira, and Curt Meuse, and to Karl Irikura for calculating the propane’s potential. This work utilized neutron scattering facilities supported in part by the National Science Foundation under Agreement No. DMR-1508249.
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Appendices
Appendix 1
1.1 Relations of the Energies, Force Constants, Gaussian Widths, and Entropies
For the stretched, connected springs of Fig. 3,
where the subscript w represents properties of the weak spring on the left, and subscript s represents the properties of the strong spring on the right. F is the force, k the force constant, and Δx the distance the point of connection resides from its position at the rest point of the unconnected spring. The signs of Δxs and Δxw are opposite.
The internal energies involved in stretching each spring from its rest point so the bond can be formed are, respectively,
From Eq. 15, we know that Δxs = − (kw/ks)Δxw and, substituting for Δxs in Eq. 16, then Us = ½ (k 2w /ks) Δx 2w . Putting Δx 2w = 2Us (ks/k 2w ) into Eq. 16 and by rearranging get
which is Eq. 2 in the main text.
The quadratic potentials of Fig. 4 show the energies versus stretch position for a reactive group attached to a polypeptide and elastically restrained by it. This group has a greater probability of being at the center, unstretched position than at the ends. The quantitative probability distribution of the possible locations of the binding groups are derived next.
With the energy U of the binding group at a location Δx from the minimum of the polymer potential U is described by
where k is the Hookean force constant, Δx is the distance moved from the minimum of the potential, and U0P is the energy minimum of the polymer potential. For the remainder of this derivation, we assign the value of U0P = 0. To simplify the appearance of the equations, from now on, x is used in place of Δx.
The normalized probability distribution of the population over the parabola is
where kB is the Boltzmann constant, and k the force constant. This is a Gaussian centered at the energy minimum. This Gaussian distribution can be characterized by its standard deviation. By comparing Eq. 19 to the general equation for a normalized Gaussian distribution
shows that the Gaussian’s characterizing width
Applying Eq. 21 for both springs of Fig. 4 at the same kBT, we can find the three equalities of Eq. 22
The σ values are a measure of 1-D displacement, so ΔS = − R ln (σw/σs) expresses the entropy change between the site before the bond is formed and when bonded. In addition, Eqs. 21 and 22 show that if the force constant changes, so does the width. So the protein’s structural entropy can be changed by stiffening the tether. Possible molecular mechanisms to do so include structuring the chain by intrachain hydrogen bonding or forming intramolecular bonds or bonding with adjacent molecules to shorten or strengthen the polymer spring.
In three dimensions, this change in σ transforms to a difference in accessible volume. For a reaction of bond formation, let the smaller, bonded volume accessible be V1, and the initial, larger unbonded accessible volume be V2. Then,
which appears as Eqs. 3 and 10a and 10b. This result only holds for the quadratic approximation for a continuum system for each binding group [83] and the approximation of homogeneous distributions within the volumes. As the attachment becomes looser, such as on a “long” unstructured polypeptide, the gaussian distribution may need to be explicitly included.
Appendix 2
2.1 Another Experimental Example of Fast Bond Formation
Another experimental example for bond formation times (compared to relatively slow mass migration) is for bonds between gold atoms, where the preorganization is fulfilled by the proximity of weak clusters of Au(CN) −2 in water. Kim et al. [201] used femtosecond x-ray scattering to follow photoactivated bond formation between the gold atoms that reside at van der Wall distances within these Au(CN) −2 clusters. The bond formation occurred within about a picosecond over which time three adjacent golds having distances of 3.9 Å and 3.3 Å from the central gold and forming a 101° angle transformed to a linear structure with both bond distances 2.8 Å. (This bond-forming process is surprisingly fast when we realize the characteristic diffusion distance over that time at ambient temperature is around 0.6 Å.) This measurement of the bond-forming supports the fraction-of-an-Angstrom motion of bond formation/breaking in solution.
Appendix 3
3.1 More About Separating Entropy and Enthalpy and the Importance of k B T
At the end of Sect. 2.3, it was noted that molecular structures can be altered by energies less than kBT—an entropic mechanism—or altered by energies greater than kBT that contribute enthalpy. For the quantitative support of that description, I will be switching back and forth between molecular lengthscale descriptions and descriptions using terms that ordinarily only apply to macroscopic systems. When descriptions involve molecular characteristics such as vibrational modes, the description should be interpreted as being that of a single molecule, which resides in a form that is an average of the ensemble from which the molecule is taken. Similarly, since a single molecule is assumed to represent the ensemble average, entropy will be used for single-molecule differences that are due to entropy on the macro scale. In addition, when thermodynamic terms are used on the molecular scale, enthalpy has no clear meaning since pressure-volume (PV) work is part of the enthalpy. Nevertheless since free energy involves both the enthalpy and entropy, let us use enthalpy as the term and ignore the difference between internal energy and enthalpy.
To clarify the nature of entropy, consider a protein residing in its equilibrium form that exhibits many low energy vibrations [202] (i.e., < 200 cm−1 at 25 °C). Now add some energy within a few ps [42, 101, 203]. The added energy first partitions among these same vibrational modes and eventually also migrates and adds to the solvent’s vibrations, rotations, and translations that define the temperature. The added energy is eventually distributed in a volume so large relative to the protein that the temperature can be considered unchanged. This added energy cannot be recovered because no temperature difference remains which would be able to drive some energy back to, e.g., change the molecule’s structure. The energy distributed to these low-energy modes of the protein and of the water is, then, the entropic part; the entropy is the energy “dispersed” or “dissipated,” [204] which are useful terms to describe the progression of events described in this paragraph.
On the other hand, if the work going into the molecule is distributed into modes that are not occupied at kBT (say, arbitrarily, 10 kBT) or changes the Boltzmann occupancy of some modes at lower energies but still greater than kBT, then the energy put in can be recovered by removal from the same modes, which drops the molecular energy to lower states. This energy can be recovered since the temperatures of those modes—as characterized by the Boltzmann distribution—are greater than the surroundings, which allows the energy to flow back. This recoverable energy is the enthalpic part.
While energy added to the protein can flow into modes that can be characterized as either entropic or enthalpic, the delineation between the two is not sharp [189]. The reason the boundary remains indistinct is that while the ambient temperature is the dividing line, the Boltzmann distribution indicates that energy states greater than kBT are also occupied at the system temperature. (As mentioned earlier, a state with energy kBT above ground is 37% as populated as the ground state, and one at 2kBT is 14% as populated.) As a result, some normally unrecoverable energy (when ΔT = 0) can be recoverable by removing energy from the partially occupied higher-energy states. This blurring in energy may be reasonably assumed to be about 3 kBT wide. If no states exist in that range, the enthalpy-entropy separation is sharp. For a protein in solution, this sharp separation is not possible.
One reason for this impossibility is that the longer the length scale of a vibration, the lower the vibrational energy levels that are available in the (molecule + solvent). This relationship can be seen in column 3 of Table 1. The lower energy vibrations are associated with larger groups of bonded atoms: examples are librations of groups of four atoms and vibrations that occur over so many atoms they are classified as acoustic modes [205,206,207]. This lengthscale-frequency relationship brings us full circle to the differences between distorting alkane chains being enthalpic (propane) and entropic (polyethylene) as discussed in Sect. 2.2. The long chain has low energy vibrational modes that can be excited by the random thermal motions of the surroundings. The short chain can have only the methyl rotations excited this way. The indistinct boundary between enthalpy and entropy is confirmed since chains with lengths greater than propane decrease the enthalpic contribution, and shortening the polyethylene eventually increases the enthalpic contribution until reaching some length of chain that has both mechanisms contributing equally to the restoring force. The boundary of enthalpic and entropic contributions is indistinct.
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Rubinson, K.A. Why Proteins are Big: Length Scale Effects on Equilibria and Kinetics. Protein J 38, 95–119 (2019). https://doi.org/10.1007/s10930-019-09822-x
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DOI: https://doi.org/10.1007/s10930-019-09822-x