The endocannabinoid hydrolase FAAH is an allosteric enzyme
Faculty of Biosciences, and Technology for Food Agriculture and Environment, University of Teramo, Teramo, Italy
European Center for Brain Research (CERC)/Santa Lucia Foundation, Rome, Italy
Faculty of Veterinary Medicine, University of Teramo, Teramo, Italy
Barcelona Biomedical Research Park (PRBB), University of Pompeu Fabra and Icrea, Barcelona, Spain
Department of Experimental Medicine and Surgery, Tor Vergata University of Rome, Rome, Italy
Department of Medicine - Campus Bio-Medico University of Rome, Rome, Italy
Abstract
Fatty acid amide hydrolase (FAAH) is a membrane-bound homodimeric enzyme that in vivo controls content and biological activity of N-arachidonoylethanolamine (AEA) and other relevant bioactive lipids termed endocannabinoids. Parallel orientation of FAAH monomers likely allows both subunits to simultaneously recruit and cleave substrates. Here, we show full inhibition of human and rat FAAH by means of enzyme inhibitors used at a homodimer:inhibitor stoichiometric ratio of 1:1, implying that occupation of only one of the two active sites of FAAH is enough to fully block catalysis. Single W445Y substitution in rat FAAH displayed the same activity as the wild-type, but failed to show full inhibition at the homodimer:inhibitor 1:1 ratio. Instead, F432A mutant exhibited reduced specific activity but was fully inhibited at the homodimer:inhibitor 1:1 ratio. Kinetic analysis of AEA hydrolysis by rat FAAH and its F432A mutant demonstrated a Hill coefficient of ~1.6, that instead was ~1.0 in the W445Y mutant. Of note, also human FAAH catalysed an allosteric hydrolysis of AEA, showing a Hill coefficient of ~1.9. Taken together, this study demonstrates an unprecedented allosterism of FAAH, and represents a case of communication between two enzyme subunits seemingly controlled by a single amino acid (W445) at the dimer interface. In the light of extensive attempts and subsequent failures over the last decade to develop effective drugs for human therapy, these findings pave the way to the rationale design of new molecules that, by acting as positive or negative heterotropic effectors of FAAH, may control more efficiently its activity.
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Subject terms: Enzymes, Enzyme mechanisms
Article notes
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Received 2019 Sep 26; Accepted 2020 Jan 22; Collection date 2020.
Introduction
Endocannabinoids form a relevant class of lipids that are widespread in tissues, where they exert diverse biological actions1. Endocannabinoids have been demonstrated to reduce pain and inflammation, modulate energetic homeostasis and appetite, and have anticancer, anxiolytic, and neuroprotective effects through type-1 and/or type-2 cannabinoid receptors (CB1 and CB2), as well as via stimulation of transient receptor potential vanilloid channels, peroxisome proliferator-activated receptors, and additional targets2–4. Their degradation is due to the activity of several metabolic enzymes, among which FAAH has a prominent role also in vivo5. In addition, biotransformation of endocannabinoids is catalysed by lipoxygenases (LOXs) or cyclooxygenase-2 (COX-2)6–8.
FAAH is a membrane-bound homodimer that is able to hydrolyse AEA and, to a lesser extent, 2-arachidonoylglycerol (2-AG), N-oleoylethanolamine9,10, N-palmitoylethanolamine11, and N-oleoyltaurine5,12,13. The biological activity of AEA, 2-AG and related compounds within the central nervous system2,3 and at the periphery has been recently reviewed6.
The 3D structures of a truncated form of rat FAAH lacking the N-terminal region14 (hereafter referred to as rFAAH), and of its humanized form containing residues of the human active site15, have been resolved at high resolution, and some details of the catalytic mechanism of the enzyme have been disclosed16,17. In particular, details of substrate selection have been elucidated, leading to the general consensus that structural flexibility of FAAH is a key factor18,19.
The crystallographic structure shows that rFAAH is a homodimer, where a transmembrane hydrophobic domain anchors each monomer to the lipid bilayer with a parallel orientation20. Indeed, each subunit contains at least two channels, one for the entry of hydrophobic substrates from the membrane side, and the other for the exit of hydrophilic products through a cytosolic gate14,16.
Increasing the concentration of endocannabinoids through the inhibition of FAAH has been considered a valuable therapeutic approach to enhance their antinociceptive and anti-inflammatory effects, as well as to protect the nervous system against exogenous insults18,21–23. However, extensive attempts over the last decade and subsequent failures to develop clinically effective drugs for human therapy24–26 suggest that FAAH is a complex target enzyme. It has been proposed that the parallel orientation of FAAH monomers could in principle allow simultaneous recruitment of two molecules of substrates from the same membrane side15,16, but the question of whether a functional communication exists between FAAH monomers leading to an allosteric modulation of the enzyme has remained as yet unanswered.
To interrogate such a possibility, here we analyzed the catalytic properties of rFAAH and two of its mutants, as well as of a full length human FAAH (hFAAH). One of rFAAH mutants (F432A) contains a single substitution known to reside in the active site and proposed to act as a dynamic modulator by in silico analysis27,28. The other mutant (W445Y) carries a single substitution in a region known to be involved in dimer stabilization29. We show that full inhibition of enzyme activity is achieved in rFAAH, its F432A mutant and hFAAH, when only one of the two active sites of the enzyme is occupied by different prototypical inhibitors. Additional kinetic analysis and molecular dynamics simulation further demonstrated that all these FAAHs behave as allosteric enzymes. Instead, the W445Y mutant of rFAAH was not inhibited when half of the active sites were occupied by the same inhibitors, nor did it show an allosteric kinetics. It can be concluded that W445 plays a key role in inter-subunit communication, thus supporting the presence of functional cooperativity. The allosteric control of FAAH implies a fine tuning of its activity within the cell, and opens the possibility to discover and design new non-substrate molecules that, targeting heterotropic allosteric sites of FAAH, can modulate enzyme activity, and potentiate or attenuate the efficacy of FAAH inhibitors.
Results
Functional communication between FAAH monomers
A canonical manner to assess an allosteric behaviour of an enzyme is to ascertain the presence of a functional communication between its monomers. To this end, in the case of a homodimer enzymatic activity can be analysed at two homodimer:inhibitor stoichiometric ratios, whereby the inhibitor binds both active sites (1:2 ratio) or one only (1:1 ratio)30.
The specific enzymatic activity of rFAAH was reduced almost completely (>95%) using the selective and irreversible FAAH inhibitor 3′-carbamoyl-[1,1′-biphenyl]-3-yl cyclohexylcarbamate (URB597)31 at a homodimer:inhibitor molar ratio of 1:2 (Fig. 1b). Interestingly, the same reduction of rFAAH specific activity was obtained also at a homodimer:URB597 ratio of 1:1 (Fig. 1b). Also other widely used FAAH inhibitors, like the irreversible blockers methoxyarachidonoyl fluorophosphonate (MAFP)14, N-phenyl-4-(quinolin-3-ylmethyl)piperidine-1-carboxamide (PF-750)15 and N-pyridin-3-yl-4-[[3-[5-(trifluoromethyl)pyridin-2-yl]oxyphenyl]methyl]piperidine-1-carboxamide (PF-3845)32, and the reversible blockers 7-phenyl-1-(5-pyridin-2-yl-1,3-oxazol-2-yl)heptan-1-one (OL-135)33 and 1-biphenyl-4-ylethenyl piperidine-1-carboxylate (ST4070)34 showed the same effects as URB597 at both molar ratios (Tables 1 and 2). Of note, similar inhibitions of hFAAH were observed with the same blockers at the same homodimer:inhibitor molar ratios used for rFAAH (Tables 1 and 2).
| rFAAH (% of specific activity) | hFAAH (% of specific activity) | |
|---|---|---|
| CTRL | 100.0 ± 4.2§ | 100 ± 1.0# |
| URB597 | 3.5 ± 0.8*** | 36 ± 2.0** |
| MAFP | 2.0 ± 0.5*** | 0.31 ± 0.01*** |
| PF-750 | 2.9 ± 0.3*** | 53 ± 11** |
| PF-3845 | 1.9 ± 0.6*** | 0.24 ± 0.01*** |
| OL-135 | 4.3 ± 0.9*** | 62 ± 8** |
| ST4070 | 4.3 ± 1.3*** | 68 ±` 4** |
| rFAAH (% of specific activity) | hFAAH (% of specific activity) | |
|---|---|---|
| Control | 100.0 ± 4.2§ | 100 ± 1.0# |
| URB597 | 2.3 ± 1.3*** | 23.0 ± 3.0** |
| MAFP | 3.5 ± 0.4*** | 5.0 ± 9.0** |
| PF-750 | 3.6 ± 0.2*** | 49.0 ± 3.0** |
| PF-3845 | 3.8 ± 0.2*** | 2.0 ± 3.0*** |
| OL-135 | 6.8 ± 1.0*** | 59.0 ± 12.0** |
| ST4070 | 6.9 ± 0.5*** | 64.0 ± 17.0** |
The amino acid F432 is in the active site of FAAH, where it is involved in activation of the AEA substrate with a pivotal role for substrate hydrolysis27. Here, the F432A rFAAH mutant showed a markedly reduced (by half) specific activity compared to the wild-type enzyme (Fig. 1b). Much alike rFAAH, at a 1:1 homodimer:URB597 molar ratio F432A rFAAH mutant was fully inhibited, and so was at 1:2 ratio. These findings demonstrate that, in keeping with a position of F432 far from the monomer-monomer interface35, this residue does not contribute to monomer-monomer functional communication.
A relevant rFAAH region proposed to mediate the inter-subunit functional interaction is the area around the evolutionarily conserved residue W44529. The latter is indeed a protruding residue that makes the surrounding patch particularly rich in contacts between the two monomers. Thus, we analysed the specific activity of W445Y rFAAH mutant, alone or in the presence of URB597 at 1:2 or 1:1 homodimer:inhibitor stoichiometric ratios. Interestingly, W445Y mutation did not affect rFAAH specific activity per se, yet it led to ~50% reduction of enzyme activity at a homodimer:inhibitor ratio of 1:1, and to full inhibition at 1:2 ratio (Fig. 1b). These observations suggest that W445 is involved in the inter-subunit interaction, and that its substitution impairs monomer-monomer functional communication.
Kinetic properties of wild-type hFAAH, rFAAH, and rFAAH mutants
The same radiometric assay used to assess FAAH inhibition was used to perform kinetic analysis of the wild-type forms of human and rat FAAH (See Table 3 and Supplementary Fig. 1). The calculated Hill coefficient (nHill) values of both rFAAH and hFAAH are suggestive of a positive cooperativity of substrate hydrolysis (Table 3). The binding curve that better fits both rFAAH and hFAAH kinetics is a sigmoid obtained through nonlinear regression analysis using the Hill equation (with values of correlation coefficient R2 and χ2 of 0.9966 and 579, and of 0.9926 and 154, for rFAAH and hFAAH, respectively), with a K0.5 of 12.3 ± 3.1 µM and 8.6 ± 2.7 µM and nHill of 1.6 ± 0.3 and 1.9 ± 0.3, for rFAAH and hFAAH, respectively (Table 3). Instead, analysis of the same kinetic data through Michaelis-Menten equation yielded a poorer fitting (with values of correlation coefficient R2 and χ2 of 0.9869 and 1045, and of 0.9521 and 1064, for rFAAH and hFAAH respectively) (Supplementary Fig. 1).
| K0.5 (µM) | nHill | |
|---|---|---|
| rFAAH# | 12.3 ± 3.1 | 1.6 ± 0.3 |
| hFAAH# | 8.6 ± 2.7 | 1.9 ± 0.3 |
| rFAAH | 15.7 ± 2.2 | 1.6 ± 0.2 |
| rFAAH:URB597 (1:0.5) | 20.1 ± 3.6 | 1.6 ± 0.4 |
| rFAAH-F432A | 31.0 ± 4.8 | 1.7 ± 0.4 |
| rFAAH-W445Y | 20.0 ± 5.5 | 0.9 ± 0.2** |
We further analyzed rFAAH and its two mutants by means of a fluorogenic assay that is widely used and accepted as a convenient alternative to the radiometric method. Such a fluorogenic assay yielded similar values of the kinetic parameters of the rFAAHs (see Table 3), and was used to perform all subsequent analyses.
Even by using the fluorogenic assay, we found that the isotherm that better described rFAAH kinetics had a sigmoidal shape (Fig. 2a), that could be fitted by Hill equation (with correlation coefficient R2 and χ2 values of 0.9952 and 412, respectively) with a K0.5 of 15.7 ± 2.2 µM and a nHill of 1.6 ± 0.2 (Table 3). Instead, analysis of the same kinetic data through Michaelis-Menten equation yielded a poorer fitting (with values of correlation coefficient R2 and χ2 of 0.9869 and 1098, respectively) (Fig. 2b). The calculated nHill values of both rFAAH and hFAAH are suggestive of a positive cooperativity of substrate hydrolysis (Table 3).
At a homodimer:inhibitor ratio of 1.0:0.5, rFAAH showed a sigmoidal substrate dependence (Fig. 2c) with an increased K0.5 value and the same nHill value of those of rFAAH alone (Table 3). These results demonstrate that at a 1.0:0.5 stoichiometry, the amount of inhibitor is not enough to saturate at least one of the two active sites; thus, under these experimental conditions, the higher value of K0.5 compared to that calculated in the absence of inhibitor seems to reflect a reduced amount of inhibitor-free enzyme (Table 3).
In addition, kinetic analysis of F432A rFAAH showed a cooperative behaviour (Fig. 2d) with an increased value of K0.5 and the same nHill values as wild-type rFAAH (see Table 2). Instead, kinetic analysis of W445Y rFAAH showed a loss of cooperativity (Fig. 2e), with a sigmoidal shape and R2 and χ2 values of 0.9721 and 1144, respectively. Of note, the kinetic data of the latter mutant were better fitted by Michaelis-Menten equation, with R2 and χ2 values of 0.9910 and 387, respectively (Fig. 2f), and nHill value ~1.0 (Table 3). These findings strongly indicate that W445Y substitution completely impairs rFAAH cooperativity.
Molecular dynamics simulations
In order to have indications on the possible molecular mechanism behind the allosteric behaviour of rFAAH, we performed high-throughput molecular dynamics (MD) simulations on two systems: URB597 bound to wild-type rFAAH (URB597/rFAAH complex) and to its W445Y mutant (URB597/W445Y-rFAAH complex). Inhibition of rFAAH by URB597 occurs through cleavage of the carbamate bond of the inhibitor36, thus we modelled only the cyclohexane aminocarboxylic acid moiety of URB597 in the active site of one monomer (referred to as monomer A) of the enzyme (Fig. 3).
In the URB597/rFAAH complex we found a direct interaction between the two monomers that may explain the allosteric nature of the dimer. Indeed, in monomer A the loop comprising residues 266–275 contains an OH group (Oγ) of T274 that forms a hydrogen bond with side chain nitrogen of W445 in monomer B, and viceversa. The distance between these residues was often 2–3 Å over the entire trajectories (Fig. 3 upper panel a,b; lower panel, a-d). Instead, we failed to observe a similar interaction for URB597/W445Y-rFAAH, because distances between Y445 and T274 were >6 Å in all trajectories (Fig. 3 upper panel, d,f; lower panel, a-d).
Discussion
Our study demonstrates for the first time that FAAH — the main hydrolase cleaving AEA and related compounds — is an allosteric enzyme. There are several lines of evidence in support of this claim: (i) FAAH is composed of two identical subunits symmetrically arranged14; (ii) the wild-type enzyme is fully inhibited when only one subunit of the dimer is bound to one inhibitor molecule, but not in the W445Y mutant, where a substitution is made in the inter-subunit region (Fig. 1); (iii) kinetic analysis shows a sigmoidal dependence of FAAH-catalyzed reaction on AEA concentration, while the W445Y mutant shows a hyperbolic curve (Fig. 2); (iv) molecular dynamics simulations suggest that the mechanism of cooperativity of FAAH involves W445, which could possibly transmit the conformational change from one subunit to the other, thus controlling the active site accessibility.
Quaternary structure is a necessary, but not sufficient, condition for a protein to display allosteric properties. X-ray crystallographic studies14,15 showed that FAAH protein forms high molecular weight oligomers, but suggested the homodimer as the biological structure of both rFAAH and hFAAH. In line with this, we also found an oligomeric organization of FAAH in solution and demonstrated that FAAH oligomers are present only in small amounts (5–8%); once dissociated into homodimers (also due to stabilization by biological membranes), the latter showed the same kinetic properties as the oligomers of FAAH20. These data, together with the cooperative behaviour of FAAH reported here, indicate the FAAH homodimer as the allosteric functional unit of the enzyme.
To ascertain the possible allosteric communication between the two monomers of FAAH, we assayed the effects on its catalytic activity of selective inhibitors at a stoichiometric ratio of 1:1 with respect to the dimeric form, an approach successfully employed to demonstrate allosterism of COX-123 and COX-230,37, two enzymes with a structural topology similar to that of FAAH. Inhibition of the catalytic activity of both rFAAH and hFAAH is comparable at both homodimer:inhibitor stoichiometric ratios of 1:1 and 1:2 (Tables 1 and 2). This finding demonstrates that occupancy of one active site with the inhibitor molecule is able to impair the catalytic activity also in the other (unoccupied) active site, and strongly supports the presence of a functional cross-talk between the two subunits of FAAH.
It is noteworthy that both irreversible inhibitors (like URB597, MAFP, PF-750, PF-385), and reversible blockers (like OL-135 and ST4070) yielded the same results, suggesting that the mechanism of inhibition was not relevant. Incidentally, the different potencies of the same inhibitor on rFAAH compared to hFAAH are not unprecedented17,30, and are likely due to structural differences between the two enzymes38.
Kinetic analyses of rFAAH and hFAAH strongly support the allosteric nature of FAAH suggested by the inhibition studies. In particular, the values of Hill coefficients (Fig. 2a,b and Table 3) imply that FAAH has homotropic substrate cooperativity. Functional studies of site-directed mutant enzymes further demonstrated that F432A mutant retained homotropic substrate cooperativity, while the W445Y mutant completely lost cooperativity, confirming that the mechanism of FAAH allosterism involves W445 but not F432 (Fig. 2e,f).
In order to get additional information on the experimentally demonstrated FAAH allosterism, we performed microsecond MD simulations of rFAAH with only one URB597 molecule bound at one of the two monomers. Notably, MD simulations revealed the presence of two specific hydrogen bonds in the rFAAH homodimer (Fig. 3). In particular, for the URB597/wt-rFAAH complex, the in silico analysis suggests the presence of a stable interaction between residues W445 and T274 of both monomers.
Our MD approach showed that substitution of W445 with a tyrosine residue was sufficient to prevent the formation of the two hydrogen bonds in W445Y mutant. Unfortunately, our simulations did not allow to decipher the underlying allosteric mechanism. However, it should be noted that the position of the conserved residue W445 — fully buried within the FAAH core and located at the interface between the two subunits — makes this residue particularly suitable to propagate conformational changes from one active site of the enzyme to the other. Concerning T274, this was suggested by MD simulation as a possible interacting residue with W445, via a quite stable hydrogen bond in rFAAH. However, T274 is only conserved both in rFAAH and mouse FAAH, while in the human enzyme, at the same position, there is a glutamate (E274), a residue that could still form a hydrogen bond with W445. Thus, it can be speculated that dynamic interaction among W445 of one monomer and polar residues located in the 266–275 loop region of the other monomer (as the T274 here suggested by MD for rFAAH) could allosterically control the structure of the enzyme, thus regulating substrate accessibility to the catalytic site of FAAH. However, these mechanicistic aspects deserve to be analyzed with a more dedicated study.
Allosteric enzymes are known to be placed at key points of metabolic pathways, in order to finely regulate their fluxes according to the specific state of the cell. In line with this, it is tempting to speculate that an allosteric FAAH is suitable to finely tune intensity and duration of signalling by AEA, as well as by other bioactive fatty acid amides that are enzyme substrates, such as N-oleoylethanolamine, N-palmitoylethanolamine and N-oleoyltaurine9,10. At any rate, an allosteric regulation of FAAH emphasizes the biological relevance of this enzyme as a key controller of endocannabinoid signalling. In this context, accumulated evidence demonstrates a complex interplay among distinct FAAH substrates, and it is likely that an overall inhibition of enzyme activity can alter the spatiotemporal interactions among these bioactive lipids, and transduction pathways thereof39. For instance, promising results have been obtained by dissociating FAAH-catalysed hydrolysis of N-acylethanolamines versus N-acyltaurines through structure-guided design of a point mutant in the cytoplasmic access tunnel of the enzyme19. A similar approach has also been successfully used to design “substrate-selective” COX-2 inhibitors that prevent endocannabinoid inactivation without affecting prostaglandin generation from arachidonic acid8,40. Therefore, it is possible that also substrate preference of FAAH could change in the presence of suitable inhibitors (at a 1:1 ratio), with a clear impact on cell signalling under pathophysiological conditions.
On a final note, pharmacological and genetic augmentation of endogenous fatty acid amides is known to produce pleiotropic actions, including analgesic22, anxiolytic34, anti-inflammatory21, and anti-depressant effects41. Unsurprisingly, in the last few years FAAH has been the target of several drug development programmes, aimed at treating a broad range of human pathological conditions24. Our present data suggest that allosteric drug development could be a novel pharmacological strategy for controlling in a more selective and efficient manner the “catalytic promiscuity” of FAAH. Indeed, allosteric sites are structurally much less conserved than catalytic sites, thus supporting the development of drugs — positive or negative heterotropic modulators — with much greater selectivity. In this context two phenoxyacyl-ethanolamides, 3-n-pentadecylphenolethanolamide and cardanolethanolamide, have been described as FAAH activators42, and it can be speculated that these non-hydrolysable analogues of N-acylethanolamines may stimulate hydrolysis of AEA and congeners by acting as positive allosteric modulators of FAAH.
In conclusion, we provide unprecedented evidence for an allosteric regulation of FAAH, providing unexplored opportunities to design and develop novel therapeutic drugs targeted to regulatory site(s) of this major AEA-inactivating enzyme.
Methods
Reagents and enzymes
All chemicals were of the purest analytical grade. AEA, arachidonic acid, ethanolamine, and Protease Inhibitor Cocktail were from Sigma Chemical Co. (St. Luis, MO USA). IPTG was purchased at Promega Corporation (Wisconsin, USA). The E. coli BL21(DE3)pLysS competent cells were purchased from Merck KGaA (Darmstadt, Germany). Threalose was from Cargill (Cargill Incorporated, Minneapolis, USA). [3H]-AEA was from Larodan (LARODAN Fine Chemicals AB, Malmö, Sweden). AAMCA was from BIOMOL (BIOMOL International, USA). The Talon resin was from Clontech (California, USA). All other chemicals were purchased from Sigma Chemical Co. (Milan, Italy), unless stated otherwise.
ΔTM rFAAH was purified as reported20. In the F432A rFAAH mutant the protein codon TTT at position 1355 of cDNA was mutated into GCT resulting in the substitution of the phenylalanine in position 432 of the protein sequence with alanine. In the W445Y rFAAH mutant the codon TGG was mutated in position 1394 of the cDNA into TAC obtaining a consequent substitution of tryptophan in position 445 of the protein sequence with tyrosine. The catalytically active F432A and W445Y rFAAH mutants were expressed in Escherichia coli with a hexahistidine tag using the prokaryotic expression vector pTrcHisA, and were extracted from cell lysates according to the protocol of Patricelli et al.35 x with modifications. Briefly, the proteins were expressed in the competent cells according to the manufacturer’s guidelines. To improve the protein recovery, cell pellets were subjected to mechanical rupture using the following lysis buffer: 0.5 M Tris/HCl, pH 7.5, 0.1 M NaCl, 0.5% (w/v) CHAPS, 10% (w/v) trehalose. Lysozyme at a final concentration of 1 mg/mL and a 10 μl/mL Protease Inhibitor Cocktail were added to the lysis buffer. The resulting lysate was then sonicated with a tip sonicator (Bandelin, Berlin Germany) with three 10 s pulses (50% power), and then centrifuged at 10,000 × g for 30 min at 4 °C. Subsequently, the proteins were purified by metal affinity chromatography with the Talon cobalt affinity resin (Clontech). The column was pre-equilibrated with 10 column volumes of 0.5 M Tris/HCl, pH 7.5, 0.1 M NaCl, 10% (w/v) trehalose (column buffer) containing 10 mM imidazole and washed twice with column buffer containing 15 mM and 20 mM imidazole, respectively, for the removal of unspecifically bound proteins. Each FAAH sample was completely eluted after the addition of 3 column volumes of elution buffer (column buffer containing 200 mM imidazole). The purified enzymes were dialyzed overnight with the column buffer to completely remove imidazole and stored at −20 °C until use.
FAAH activity assay
Enzymatic activity of rFAAH, its mutants and hFAAH was assayed by measuring the release of [3H]-ethanolammine from [3H]-AEA (60 Ci/mmol) (Larodan Fine Chemicals AB, Malmo Sweden), using liquid scintillation counting according to the method of Gattinoni and coworkers43. In substrate-dependence experiments, that were performed including several data points in the low substrate concentration range, enzymatic activity of rFAAH and its mutants was assayed by means of the fluorescent-based method by Ramarao and colleagues44, by measuring the release of arachidonic acid and of the highly fluorescent 7-ammino-4-methyl coumarin (AMC) product from the non-fluorescent arachidonyl 7-ammino-4-methyl coumarin amide (AAMCA) substrate of FAAH. In preliminary experiments both methods (radiometric and fluorimetric) were found to yield the same catalytic constants, that were in keeping with literature data15,34,45. Kinetic analysis were done both in the presence and in the absence of 1-palmitoyl-2-oleyl-sn-glycero-3-phosphocholine (POPC) large unilamellar vesicles prepared as described previously46.
Protein concentration was determined spectrophotometrically, assuming a 0.1% extinction coefficient at 280 nm of ε = 1.11, as calculated from the primary structure using the ‘prot param’ tool in the expasy proteomic server (www.expasy.org). In all FAAH enzymatic assays carried out at a 1:1 homodimer:inhibitor stoichiometric ratio, 40 nm of the FAAH homodimer (i.e., with two active sites) and 40 nm of all the evaluated inhibitors were used. For the 1:2 homodimer:inhibitor stoichiometry 40 nm of FAAH and 80 nm of inhibitor concentration were used. All enzymatic assays were carried out at 37 °C using a pre-incubation time of 20 minutes of all the evaluated inhibitors with the different FAAHs before adding the substrate (final volume of 500 μL).
Kinetic parameters of the FAAH-catalyzed reaction were calculated from dose-dependence curves (0–100 μM substrate range) through nonlinear regression analysis using the software Kaleidagraph (Synergy Software). Allosteric behaviour was analysed by non-linear regression analysis of kinetic data using the Hill equation and the MWC formalism47,48.
Molecular dynamics
As previously done20, molecular dynamics studies were carried out in the presence of a POPC membrane. To better parallel these in silico data, we also evaluated the kinetic properties of FAAH in the presence and in the absence of POPC membranes. In agreement with previous data20, no differences were found in enzyme activity under the two experimental conditions (data not shown). Two replicas for each rFAAH-membrane system were prepared for molecular dynamics simulations. Membrane position was taken from the OPM database using the HTMD software and run using ACEMD49. Input coordinates of the systems were based on PDB code 1MT5, from where the inhibitor methyl arachidonoyl fluorophosphonate (MAFP), covalently bond to the catalytic nucleophile S241, was removed. The crystal structure of the FAAH-URB597 (PDB code 3LJ7) complex was used for superimposition in our URB597-bound models. The all-atom CHARMM36 force field was used for the protein, lipid and water atoms. With an identical setup also the W445Y mutation was prepared. For each complex, we performed two independent simulations of 1 μs, giving a final aggregate of 4 μs length. More details about the set-up of the inhibitor covalently bond to the protein are reported in the Supplementary Information.
Statistical analysis
Data reported in this paper are the mean (±S.D.) of at least three independent determinations, each performed in triplicate. Statistical analysis was performed by the non-parametric Mann-Whitney U test, analyzing experimental data by means of the Prism 5 program (GraphPAD Software for Science, San Diego, CA).
Supplementary information
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Acknowledgements
This work was supported by the BioStruct X-BAG project “A new player in the modulation of protein function: the biological membranes” under the EU Framework Programme grant agreement n. 283570) to E.D. and M.M., by the Italian Ministry of Health (IZS LT 14/11 RC project) to E.D., and by the Italian Ministry of Education, University and Research (competitive PRIN 2015 project) to M.M. and S.O.
Competing interests
The authors declare no competing interests.
Footnotes
Footnote Group
Contributor Information
Enrico Dainese, Email: edainese@unite.it.
Mauro Maccarrone, Email: m.maccarrone@unicampus.it.
Supplementary information
is available for this paper at 10.1038/s41598-020-59120-1.
References
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References
- 1.Piomelli D. The molecular logic of endocannabinoid signalling. Nat. Rev. Neurosci. 2003;4:873–84. doi: 10.1038/nrn1247.
- 2.Maccarrone M, Guzmán M, Mackie K, Doherty P, Harkany T. Programming of neural cells by (endo)cannabinoids: from physiological rules to emerging therapies. Nat. Rev. Neurosci. 2014;15:786–801. doi: 10.1038/nrn3846.
- 3.Lu H-C, Mackie K. An Introduction to the Endogenous Cannabinoid System. Biol. Psychiatry. 2016;79:516–525. doi: 10.1016/j.biopsych.2015.07.028.
- 4.Maccarrone Mauro, Gasperi Valeria, Catani Maria Valeria, Diep Thi Ai, Dainese Enrico, Hansen Harald S., Avigliano Luciana. The Endocannabinoid System and Its Relevance for Nutrition. Annual Review of Nutrition. 2010;30(1):423–440. doi: 10.1146/annurev.nutr.012809.104701.
- 5.Ahn K, McKinney MK, Cravatt BF. Enzymatic pathways that regulate endocannabinoid signaling in the nervous system. Chem. Rev. 2008;108:1687–707. doi: 10.1021/cr0782067.
- 6.Maccarrone M, et al. Endocannabinoid signaling at the periphery: 50 years after THC. Trends Pharmacol. Sci. 2015;36:277–96. doi: 10.1016/j.tips.2015.02.008.
- 7.Maccarrone Mauro, Dainese Enrico, Oddi Sergio. Intracellular trafficking of anandamide: new concepts for signaling. Trends in Biochemical Sciences. 2010;35(11):601–608. doi: 10.1016/j.tibs.2010.05.008.
- 8.Hermanson DJ, Gamble-George JC, Marnett LJ, Patel S. Substrate-selective COX-2 inhibition as a novel strategy for therapeutic endocannabinoid augmentation. Trends in Pharmacological Sciences. 2014;35:358–367. doi: 10.1016/j.tips.2014.04.006.
- 9.Khurshudyan M., Sadeghi J., Pasqua A., Chattopadhyay S., Myrzakulov R., Farahani H. Interacting Ricci Dark Energy Models with an Effective Λ-term in Lyra Manifold. International Journal of Theoretical Physics. 2014;54(3):749–760. doi: 10.1007/s10773-014-2266-7.
- 10.Fu Jin, Oveisi Fariba, Gaetani Silvana, Lin Edward, Piomelli Daniele. Oleoylethanolamide, an endogenous PPAR-α agonist, lowers body weight and hyperlipidemia in obese rats. Neuropharmacology. 2005;48(8):1147–1153. doi: 10.1016/j.neuropharm.2005.02.013.
- 11.Bachur, N. R., Masek, K., Melmon, K. L. & Udenfriend, S. Fatty acid amides of ethanolamine in mammalian tissues. J. Biol. Chem (1965).
- 12.Huang Susan M., Bisogno Tiziana, Petros Timothy J., Chang Sai Y., Zavitsanos Paul A., Zipkin Robert E., Sivakumar Ramachandran, Coop Andrew, Maeda Dean Y., De Petrocellis Luciano, Burstein Sumner, Di Marzo Vincenzo, Walker J. Michael. Identification of a New Class of Molecules, the Arachidonyl Amino Acids, and Characterization of One Member That Inhibits Pain. Journal of Biological Chemistry. 2001;276(46):42639–42644. doi: 10.1074/jbc.M107351200.
- 13.Di Marzo V, Maccarrone M. FAAH and anandamide: is 2-AG really the odd one out? Trends Pharmacol. Sci. 2008;29:229–33. doi: 10.1016/j.tips.2008.03.001.
- 14.Bracey MH, Hanson MA, Masuda KR, Stevens RC, Cravatt BF. Structural adaptations in a membrane enzyme that terminates endocannabinoid signaling. Science. 2002;298:1793–6. doi: 10.1126/science.1076535.
- 15.Mileni M, et al. Structure-guided inhibitor design for human FAAH by interspecies active site conversion. Proc. Natl. Acad. Sci. 2008;105:12820–12824. doi: 10.1073/pnas.0806121105.
- 16.McKinney Michele K., Cravatt Benjamin F. STRUCTURE AND FUNCTION OF FATTY ACID AMIDE HYDROLASE. Annual Review of Biochemistry. 2005;74(1):411–432. doi: 10.1146/annurev.biochem.74.082803.133450.
- 17.Palermo G, et al. Keys to Lipid Selection in Fatty Acid Amide Hydrolase Catalysis: Structural Flexibility, Gating Residues and Multiple Binding Pockets. PLOS Comput. Biol. 2015;11:e1004231. doi: 10.1371/journal.pcbi.1004231.
- 18.Boger DL, et al. Discovery of a potent, selective, and efficacious class of reversible alpha-ketoheterocycle inhibitors of fatty acid amide hydrolase effective as analgesics. J. Med. Chem. 2005;48:1849–56. doi: 10.1021/jm049614v.
- 19.McKinney MK, Cravatt BF. Structure-based design of a FAAH variant that discriminates between the N-acyl ethanolamine and taurine families of signaling lipids. Biochemistry. 2006;45:9016–22. doi: 10.1021/bi0608010.
- 20.Dainese Enrico, De Fabritiis Gianni, Sabatucci Annalaura, Oddi Sergio, Angelucci Clotilde Beatrice, Di Pancrazio Chiara, Giorgino Toni, Stanley Nathaniel, Del Carlo Michele, Cravatt Benjamin F., Maccarrone Mauro. Membrane lipids are key modulators of the endocannabinoid-hydrolase FAAH. Biochemical Journal. 2014;457(3):463–472. doi: 10.1042/BJ20130960.
- 21.Centonze D, Finazzi-Agrò A, Bernardi G, Maccarrone M. The endocannabinoid system in targeting inflammatory neurodegenerative diseases. Trends Pharmacol. Sci. 2007;28:180–187. doi: 10.1016/j.tips.2007.02.004.
- 22.Cravatt B. F., Demarest K., Patricelli M. P., Bracey M. H., Giang D. K., Martin B. R., Lichtman A. H. Supersensitivity to anandamide and enhanced endogenous cannabinoid signaling in mice lacking fatty acid amide hydrolase. Proceedings of the National Academy of Sciences. 2001;98(16):9371–9376. doi: 10.1073/pnas.161191698.
- 23.Booker L, et al. The fatty acid amide hydrolase (FAAH) inhibitor PF-3845 acts in the nervous system to reverse LPS-induced tactile allodynia in mice. Br. J. Pharmacol. 2012;165:2485–96. doi: 10.1111/j.1476-5381.2011.01445.x.
- 24.Bisogno T, Maccarrone M. Latest advances in the discovery of fatty acid amide hydrolase inhibitors. Expert Opin. Drug Discov. 2013;8:509–22. doi: 10.1517/17460441.2013.780021.
- 25.Mallet C, Dubray C, Dualé C. FAAH inhibitors in the limelight, but regrettably. Int. J. Clin. Pharmacol. Ther. 2016;54:498–501. doi: 10.5414/CP202687.
- 26.Edan G, Kerbrat A. Inhibitor of Fatty Acid Amide Hydrolase — Learning from Tragic Failures. N. Engl. J. Med. 2017;376:392–394. doi: 10.1056/NEJMc1615417.
- 27.Palermo G, Rothlisberger U, Cavalli A, De Vivo M. Computational insights into function and inhibition of fatty acid amide hydrolase. Eur. J. Med. Chem. 2015;91:15–26. doi: 10.1016/j.ejmech.2014.09.037.
- 28.Palermo Giulia, Bauer Inga, Campomanes Pablo, Cavalli Andrea, Armirotti Andrea, Girotto Stefania, Rothlisberger Ursula, De Vivo Marco. Keys to Lipid Selection in Fatty Acid Amide Hydrolase Catalysis: Structural Flexibility, Gating Residues and Multiple Binding Pockets. PLOS Computational Biology. 2015;11(6):e1004231. doi: 10.1371/journal.pcbi.1004231.
- 29.Mei G, et al. Closing the gate to the active site: effect of the inhibitor methoxyarachidonyl fluorophosphonate on the conformation and membrane binding of fatty acid amide hydrolase. J. Biol. Chem. 2007;282:3829–36. doi: 10.1074/jbc.M605653200.
- 30.Zou H, et al. Human cyclooxygenase-1 activity and its responses to COX inhibitors are allosterically regulated by nonsubstrate fatty acids. J. Lipid Res. 2012;53:1336–47. doi: 10.1194/jlr.M026856.
- 31.Mor M, et al. Cyclohexylcarbamic acid 3’- or 4’-substituted biphenyl-3-yl esters as fatty acid amide hydrolase inhibitors: synthesis, quantitative structure-activity relationships, and molecular modeling studies. J. Med. Chem. 2004;47:4998–5008. doi: 10.1021/jm031140x.
- 32.Ahn K, et al. Discovery and characterization of a highly selective FAAH inhibitor that reduces inflammatory pain. Chem. Biol. 2009;16:411–20. doi: 10.1016/j.chembiol.2009.02.013.
- 33.Romero FA, et al. Potent and selective alpha-ketoheterocycle-based inhibitors of the anandamide and oleamide catabolizing enzyme, fatty acid amide hydrolase. J. Med. Chem. 2007;50:1058–68. doi: 10.1021/jm0611509.
- 34.Butini S, et al. Discovery of Potent Inhibitors of Human and Mouse Fatty Acid Amide Hydrolases. J. Med. Chem. 2012;55:6898–6915. doi: 10.1021/jm300689c.
- 35.Patricelli MP, Lashuel Ha, Giang DK, Kelly JW, Cravatt BF. Comparative characterization of a wild type and transmembrane domain-deleted fatty acid amide hydrolase: identification of the transmembrane domain as a site for oligomerization. Biochemistry. 1998;37:15177–15187. doi: 10.1021/bi981733n.
- 36.Mileni M, et al. Crystal Structure of Fatty Acid Amide Hydrolase Bound to the Carbamate Inhibitor URB597: Discovery of a Deacylating Water Molecule and Insight into Enzyme Inactivation. J. Mol. Biol. 2010;400:743–754. doi: 10.1016/j.jmb.2010.05.034.
- 37.Dong L, Sharma NP, Jurban BJ, Smith WL. Pre-existent asymmetry in the human cyclooxygenase-2 sequence homodimer. J. Biol. Chem. 2013;288:28641–55. doi: 10.1074/jbc.M113.505503.
- 38.Di Venere A, et al. Rat and human fatty acid amide hydrolases: overt similarities and hidden differences. Biochim. Biophys. Acta. 2012;1821:1425–33. doi: 10.1016/j.bbalip.2012.07.021.
- 39.Long JZ, LaCava M, Jin X, Cravatt BF. An anatomical and temporal portrait of physiological substrates for fatty acid amide hydrolase. J. Lipid Res. 2011;52:337–344. doi: 10.1194/jlr.M012153.
- 40.Hermanson DJ, et al. Substrate-selective COX-2 inhibition decreases anxiety via endocannabinoid activation. Nat. Neurosci. 2013;16:1291–1298. doi: 10.1038/nn.3480.
- 41.Wang Y, Zhang X. FAAH inhibition produces antidepressant-like efforts of mice to acute stress via synaptic long-term depression. Behav. Brain Res. 2017;324:138–145. doi: 10.1016/j.bbr.2017.01.054.
- 42.Faure L, et al. Synthesis of Phenoxyacyl-Ethanolamides and Their Effects on Fatty Acid Amide Hydrolase Activity. J. Biol. Chem. 2014;289:9340–9351. doi: 10.1074/jbc.M113.533315.
- 43.Gattinoni S, et al. Enol carbamates as inhibitors of fatty acid amide hydrolase (FAAH) endowed with high selectivity for FAAH over the other targets of the endocannabinoid system. ChemMedChem. 2010;5:357–60. doi: 10.1002/cmdc.200900472.
- 44.Ramarao MK, et al. A fluorescence-based assay for fatty acid amide hydrolase compatible with high-throughput screening. Anal. Biochem. 2005;343:143–51. doi: 10.1016/j.ab.2005.04.032.
- 45.Roughley SD, et al. Fatty acid amide hydrolase inhibitors. 3: tetra-substituted azetidine ureas with in vivo activity. Bioorg. Med. Chem. Lett. 2012;22:901–6. doi: 10.1016/j.bmcl.2011.12.032.
- 46.Dainese E, et al. A novel role for iron in modulating the activity and membrane-binding ability of a trimmed soybean lipoxygenase-1. FASEB J. 2010;24:1725–1736. doi: 10.1096/fj.09-141390.
- 47.Monod Jacque, Wyman Jeffries, Changeux Jean-Pierre. On the nature of allosteric transitions: A plausible model. Journal of Molecular Biology. 1965;12(1):88–118. doi: 10.1016/S0022-2836(65)80285-6.
- 48.Dainese Enrico, Di Muro Paolo, Beltramini Mariano, Salvato Benedetto, Decker Heinz. Subunits composition and allosteric control in Carcinus aestuarii hemocyanin. European Journal of Biochemistry. 1998;256(2):350–358. doi: 10.1046/j.1432-1327.1998.2560350.x.
- 49.Harvey MJ, Giupponi G, Fabritiis G. De. ACEMD: Accelerating Biomolecular Dynamics in the Microsecond Time Scale. J. Chem. Theory Comput. 2009;5:1632–9. doi: 10.1021/ct9000685.