Daniel
Holub
a,
Tomáš
Kubař
ab,
Thilo
Mast
a,
Marcus
Elstner
ac and
Natacha
Gillet
*ad
aDepartment for Theoretical Chemical Biology, Institute for Physical Chemistry, Karlsruhe Institute for Technology, Kaiserstr. 12, 76131, Karlsruhe, Germany. E-mail: natacha.gillet@kit.edu
bCentre for Functional Nanostructures (CFN), Karlsruhe Institute for Technology, Kaiserstr. 12, 76131, Karlsruhe, Germany
cInstitute of Biological Interfaces (IGB2), Karlsruhe Institute for Technology, Kaiserstr. 12, 76131, Karlsruhe, Germany
dInstitut de Génétique et de Biologie Moléculaire et Cellulaire (IGBMC), Institut National de La Santé et de La Recherche Médicale (INSERM), U1258/Centre National de Recherche Scientifique (CNRS), UMR7104/Université de Strasbourg, 67404 Illkirch, France
First published on 14th May 2019
Photolyases (PL) and cryptochromes (CRY) are light-sensitive flavoproteins, respectively, involved in DNA repair and signal transduction. Their activation is triggered by an electron transfer process, which partially or fully reduces the photo-activated FAD cofactor. The full reduction additionally requires a proton transfer to the isoalloxazine ring. In plant CRY, an efficient proton transfer takes place within several μs, enabled by a conserved aspartate working as a proton donor, whereas in E. coli PL a proton transfer occurs in the 4 s timescale without any obvious proton donor, indicating the presence of a long-range proton transfer pathway. Unexpectedly, the insertion of an aspartate as a proton donor in a suitable position for proton transfer in E. coli PL does not initiate a transfer process similar to plant CRY, but even prevents the formation of a protonated FAD. In the present work, thanks to a combination of classical molecular dynamics and state-of-the-art DFTB3/MM simulations, we identify a proton transfer pathway from bulk to FAD in E. coli PL associated with a free energy profile in agreement with the experimental kinetics data. The free energy profiles of the proton transfer between aspartate and FAD show an inversion of the driving force between plant CRY and E. coli PL mutants. In the latter, the proton transfer from the aspartate is faster than in plant CRY but also thermodynamically disfavoured, in agreement with the experimental data. Our results further illustrate the fine tuning of the electrostatic FAD environment and the adaptability of the FAD pocket to ensure the divergent functions of the members of the PL-CRY family.
The major role of CRY is in the regulation of diverse biological responses as a signalling molecule. CRY contributes to the entrainment of the circadian rhythm,3 the space orientation by interaction with the Earth's magnetic field1,2,4,5 (which was especially shown for the avian CRY46), and the regulation of growth or flowering state in plants.7,8 Therefore, the formation of a radical pair is required and is initiated by an ET reducing FADox to FAD˙−. Additionally, further proton transfer (PT) reactions can form FADH˙ in the presence of proton donors. Hence, CRY offers a FAD pocket with an environment supporting FAD to switch between redox states.
The main task of PL is the repair of photo-induced DNA damages by a ET between the photo-activated FADH− and the DNA lesion. Then, a backward ET occurs from the repaired thymines to the FADH˙ semiquinone to close the catalytic cycle. Consistently, the protonated FAD states (FADH˙ semiquinone or FADH− hydroquinone) prevail in PL in vivo,1 even though the oxidized FADox and its full reduction are obtained in vitro.
This FAD pocket is conserved in most PCF proteins to a large extent,9 however, it is still supposed to offer different interaction patterns to enable the different functions. For instance, a FAD˙− or FADH˙ radical needs to be formed in CRY while a FADH− needs to be stabilized in PL. Accordingly, one specific amino acid in a position close to the N5 of FAD differs between members of the PCF: in most plant CRY, e.g. CRY I from Arabidopsis thaliana (CRYI), an aspartate (Asp) is found in this position,10,11 but a non-titratable residue is often present, such as a cysteine (Cys) in entomic CRY.12 In CRY-DASH of a cyanobacterium,13 which shows a high similarity in structure and function to the PL, an asparagine (Asn) is found at this position. This homologous Asn is also present in PL, e.g. in PL from E. coli14 and A. nidulans.15 The impact of this amino acid has been studied by experimental site-directed mutagenesis, showing that it affects the behaviour of the proteins decisively: in CRYI, the Asp acts as a proton donor to form FADH˙ from a photo-reduced semiquinone FAD˙−, whereas a mutation of Asp into Cys, inspired by the entomic CRY, prevents FAD protonation.16 The mutation into Asn leads to the formation of FADH˙ despite the lack of an obvious proton donor such as Asp, which indicates the presence of an alternative PT pathway. Additionally, in the Asp to Asn mutant, a PL-like DNA repair activity was observed, which in fact requires the stabilization of FADH−.10 Conversely, the presence of Cys in entomic CRY, like in Drosophila melanogaster CRY, inhibits the protonation of FAD˙−.17,18 In this CRY, the mutation of the Cys into Asp, albeit offering a suitable proton donor to FAD, does not lead to the formation of FADH˙.19 In contrast, a mutation of Cys into Asn leads to stabilization of protonated FADH˙, which does not affect the photoreceptor function.19
In E. coli and A. nidulans PL, like in the entomic CRY, the mutation of Asn into Asp does not enable a PT to form FADH˙.20,21 After photo-reduction, the E. coli PL Asn to Asp mutant (PL-N378D) shows a slightly different UV-vis absorption spectrum compared to the spectrum for FAD˙−. It is characteristic of the presence of a different FAD state, called FADx, and the absence of FADH˙. It was hypothesized that this state indicates a strong hydrogen bond network between Asp and FAD N5 or a short-lived FADH˙.20 So, the presence of Asp blocks the stabilization of FADH˙ and furthermore inhibits any other PT pathway. Combined spectroscopic and computational studies on E. coli PL (WT-PL) showed that a strong hydrogen bond between FADH− and Asn378 stabilizes the FADH− state, which is essential for the repair activity.22,23 Further experimental studies investigated the replacement of Asn by Ser in the E. coli PL and a drop of the in vitro DNA repair activity from 50% for WT to less than 1% is observed.24 This underlines the dominant role of Asn in DNA repair, likely by stabilizing the FADH˙ and FADH− states over other redox states.
In summary, the reported observations highlight the fine tuning of the structure of the FAD pocket to stabilize the active form of the protein.25 It appears that the nature of the residue interacting with FAD N5, which may be Asp, Asn or Cys, is strongly related to the most relevant FAD protonation state in WT, and thus to the biological role of the respective protein. However, a mutation of this residue does not necessarily result in a functional conversion of the mutants. It appears that other structural or dynamical parameters, like the formation of a PT pathway, can influence the protonation/redox state of FAD.
To explore these other parameters, Müller et al. studied the protonation of FAD in WT-PL in vitro by preparing a protein which contained FAD in its fully oxidized state, FADox. The timescale of the ET to form FAD˙− was below 300 ps, and that of the subsequent PT was 4 s (see the mechanism in Fig. 1).20 Since Asn cannot protonate FAD directly, a pathway has to exist, which seems to not involve other acidic residues in the FAD pocket.13 Damiani et al. suggested that water molecules can enter the FAD pocket and form a PT pathway from the bulk water to FAD.21 The formation of the FADx state occurs in 3.3 μs in PL-N378D. Compared to this, spectroscopic studies in CRYI show that the photo-reduction of FADox occurs within 31 ps, the subsequent PT from Asp396 to FAD˙− occurs in 1.7 μs, while the backward transfer is two orders of magnitude slower (690 μs).26,27 So, the CRYI pocket allows a faster switch between protonated and deprotonated FAD than the PL pocket.
![]() | ||
Fig. 1 Comparison of the FAD˙− protonation in E. coli PL-WT, N378 mutant of PL and CRYI. The nature of the proton donor is given wherever identified; otherwise B stands for a generic proton donor. The FAD binding pocket of PL-N378D and CRYI is shown with amino acids colored in white (non-polar), green (polar) and red/blue (acidic/basic). The isoalloxazine ring of FAD and the side chains of Asp378/396 and Glu363 or Met381 are displayed explicitly. Purple dashed lines indicate hydrogen bonds between N5 of FAD and Asp378/396. Pictures of all the proteins are obtained using VMD.32 |
Computational chemistry methods provide a consistent and comparatively cheap approach to investigate the effect of differences at a molecular level between the FAD pockets from CRYI, PL-WT and mutants. In our previous study,28 we computed rate constants for both ET29–31 and PT28 processes in CRYI in agreement with the experimental results. The aim of the current study is to resolve the mechanism and energetics of the PT processes taking place in PL-WT and PL-N378D, and compare to those in CRYI (see Fig. 1). The combination of QM/MM free energy calculations of the PT and classical MD simulations provide a complete picture of the interplay between the FAD protonation and the structural and dynamical behaviour of the FAD binding pocket.
For PL-N378D, two different starting structures were created containing different protonation states of Glu363. This residue has a calculated pKa value of 6 (according to PROPKA3.1 results), which suggests the coexistence of both the protonated and the deprotonated states at physiological pH. The Glu363 side chain can interact with the carboxyl group of Asp378 and the surrounding solvent molecules. Hence, different interaction patterns with the carboxyl group of Asp378 would result from these states: a protonated Glu363 is able to form a strong hydrogen bond with negatively charged Asp378, and a weaker one with neutral Asp378; a deprotonated Glu363, however, leads to the destabilization of the deprotonated Asp378 by electrostatic repulsion. In the PL-WT simulations, this residue is deprotonated.
All of the simulations were performed with the AMBER-SB99-ILDN force field37,38 using GROMACS 5.0.4.39,40 The cofactors FAD and MTHF were parameterized with the xLeap module of AmberTools41 employing the general Amber force field (GAFF).37,42 The atomic charges of FAD, FAD˙− and FADH˙ were fitted on the electrostatic potential (RESP)43,44 obtained at the HF/6-31G*45,46 level of theory with GAUSSIAN09.47 The protein was placed in a periodic box sized 96 × 94 × 121 A3 for WT-PL and PL-N378D and 98 × 98 × 98 Å3 for CRYI. The box was filled with TIP3P water molecules to obtain a density of 1000 kg m−3, and an appropriate number of water molecules were substituted by sodium ions to achieve electroneutrality; no extra salt was added. These systems were equilibrated by means of a protocol consisting of a series of energy minimization, NVT (1 ns) and NPT (1 ns), simulations. The eventual production simulations used the Nosé–Hoover thermostat48 and the Parrinello–Rahman barostat49 to maintain a temperature of 300 K and a pressure of 1 bar, respectively. The simulations employed a leap-frog integrator with a time step of 2 fs. We performed MD simulations containing FADox (100 ns) for the PL-WT, PL-N378D and CRYI. Then, we used the final geometry from these simulations to start 50 ns MD simulations for PL-N378D and CRYI containing FAD˙−. Suitable conformations for PT are obtained in a few ns, but we extended these simulations to 200 ns to check the stability of the different interactions. For PL-WT, in order to explore the various structural consequences of FAD photo-reduction, 10 snapshots were extracted from the first simulation with FADox. They were used as the starting points for 50 ns MD simulations with FAD˙−. Here, a number of parallel runs are preferred to a single longer simulation because we had no preliminary idea about the PT pathway and we wanted to decrease the probability to sample a system trapped in a deep well where no PT pathway can be formed.
In PL-WT, the free energy profile of the PT reaction along the water wire in the protein pocket was obtained with an US-DFTB3/MM simulation. The QM region consisted of the isoalloxazine ring of FAD (the D-ribitol tail is replaced by a methyl group), the side chain of Glu106 and five water molecules. The reaction coordinate for the long-range PT in PL-WT involves the N5 of FAD˙−, the atoms of the water wire and the external proton donor, so we used the modified centre of excess charge (mCEC) by König et al.:60
![]() | (1) |
![]() | (2) |
![]() | (3) |
In PL-N378D, the free energy profile of the PT reaction between N5 of FAD and Asp378 was also obtained with a DFTB3/MM using an umbrella sampling approach. The QM region contained the side chain of Asp378 and the isoalloxazine core of FAD. The reaction coordinate for the PT involves the antisymmetric linear combination of the H–O distance of Asp378 and the H–N5 distance of FAD˙−, dO–H–N. These simulations were performed for the three protein variants involving a protonated Glu363, a deprotonated Glu363 or a methionine in position 363. Harmonic biasing potentials with a force constant of 239 kcal mol−1 Å−2 were applied, and the simulation at 300 K of each of the 20 windows was extended to 300 ps with a timestep of 0.5 fs. The free energy profile of the PT in CRYI is taken out from a previous study,28 in which the distance between the proton and the N5 of FAD, dH–N, was considered as a reaction coordinate.
Rate constants were estimated from the energy barrier heights in the free energy profiles by applying the transition state theory, using the relation61
![]() | (4) |
![]() | (5) |
ΔECoul = ECoul([ASP−–FADH˙]) − ECoul([ASPH–FAD˙−]) | (6) |
• The rotation of the Asn378 side chain to face FAD-N5: in the initial state, the keto group faces N5, after a rotation of the amino group of Asn (7 occurrences). In this conformation, mentioned as the N-conformation in Fig. 2, no interaction is observed between Asn378 and Glu363. No reverse rotation was observed (more details are provided in Fig. S1 in the ESI†).
• A flow of water molecules into the FAD pocket, also facing the FAD N5 atom (2 occurrences) while Asn378 stays in the O-conformation (see also Fig. S2 in the ESI†).
In the remaining MD simulation, Asn378 stays in the O-conformation but no water comes into the pocket.
Analogous MD simulations were carried out for PL-N378D and CRYI in the FADox state and then 200 ns MD simulations were carried out in the FAD˙− state. During the MD simulations with FADox, the protonated Asp378/396 backbone carbonyl oxygen faces FAD N5, which prevents any proton transfer. After the switch from FADox to FAD˙−, the Asp residue rotates within a few nano-seconds in both proteins: the protonated side chain now faces the O4 or N5 of FAD and forms a hydrogen bond (see the ESI,† Fig. S3). This conformation is a prerequisite for a potential PT to FAD˙−. The distance between FAD N5 and the proton of Asp378/396 was measured along the MD trajectories of both PL-N378D and CRYI, as were the distances between FAD and several neighbouring amino acid side chains (shown in Table S1, ESI†).
![]() | ||
Fig. 3 The different steps for the reduction of FADox to FADH˙ in E. coli PL-WT and their characteristic times obtained from experiments (in black) or computation (red). |
To better characterise the kinetics of this event, free energy profiles were computed for the water molecules entering the FAD pocket. We used classical force field simulations in combination with US. To reduce the complexity of the possible reorientations in the pocket, we focused on the free energy barrier for the entrance of two water molecules: (I) the reaction coordinate for the entrance of the first water molecule is the distance of this water molecule from FAD; (II) the reaction coordinate for the second water molecule is the distance of this water molecule from the first water molecule. The resulting free energy profiles are shown in Fig. 5(I) and (II).
The first water molecule has to overcome a rather low barrier of 3.5 kcal mol−1 corresponding to a rate of ktrans ≈ 18 ns−1, finding a stable minimum in the binding pocket. The second water molecule has to overcome a similar barrier but the final state is not thermodynamically stable, indicating that the formation of this water wire is a transient process. These two water molecules form a path connecting FAD N5 with a potential proton donor outside the FAD pocket. Inspection of the structure identifies Glu106 as the closest titratable amino acid (Fig. 6). QM/MM US simulations were performed, considering the Glu106 side chain, FAD˙− and the five water molecules as possible proton carriers in the QM region. Since the formation of the water wire is a transient phenomenon, we had to constrain the water position in order to compute the free energy profile for PT from Glu106 to FAD. The resulting free energy profile is shown in Fig. 6.
The first barrier of 19 kcal mol−1 is associated with the proton transfer from Glu106 to the water wire. The transfer of the proton to the first water molecule carries an energy penalty of 12.5 kcal mol−1, while moving the proton further to the second water molecule after crossing the first barrier leads to the first stable local minimum. The second step starts with a PT proceeding along the water wire and through the loop, from the third to the fourth water molecule, over another barrier of 7 kcal mol−1. The transfer to the fifth water molecule and then to the N5 atom of FAD is a downhill process resulting in a product state 10 kcal mol−1 below the reactant state. If we consider a pKa of 4.2 for Glu106 (pKa of glutamic acid in solution), this driving force value gives an estimation for the FAD˙− pKa around 11.5. The rate limiting step is the deprotonation of the donor with a rate constant of 0.13 s−1, which is in agreement with the experimental data.18,20
![]() | ||
Fig. 7 The individual steps of the FAD protonation by an aspartate in PL-N378D and CRYI and their experimental (black) or computational (red) time constants. |
PL-N378D | CRYI | |||
---|---|---|---|---|
ΔG≠I.→III. | (GII.–GI.) | [kcal mol−1] | 4.9 | 7.5 |
ΔG≠III.→I. | (GII.–GIII.) | [kcal mol−1] | 2.9 | 8.9 |
ΔG0 | (GIII.–GI.) | [kcal mol−1] | 2.0 | −1.4 |
ΔG0PL − ΔG0CRY | [kcal mol−1] | 3.4 | ||
k I.→III. | [ns−1] | 1.6 | 0.02 | |
k III.→I. | [ns−1] | 47 | 0.002 |
Our free-energy landscape favouring FADH˙ in CRYI is consistent with the experimentally well-defined FADH˙ spectrum. For PL-N378D, the reported measured spectrum was associated with a state called FADx, which mostly overlaps with the FAD˙− spectrum.20 This is in line with the free-energy profile, highlighting an energetically favoured FAD˙− state. Nevertheless, the activation energy for the forward and backward PT is only 4.9 kcal mol−1 and 2.9 kcal mol−1, respectively, which corresponds to rate constants of 1.6 ns−1 and 47 ns−1. So, PT is feasible during the recording time of the spectra, and a weighted superposition of both species may lead to a particular form of the absorption spectrum.
In CRYI, the FADH˙–Asp378− product is slightly favoured (the sum of ΔEcoul = −3.9 kcal mol−1), while there is no significant preference for either state in PL-N378D (sum of ΔEcoul = +0.6 kcal mol−1). It is interesting to see that the total difference in electrostatic energy of 4.5 kcal mol−1 roughly resembles the difference in the reaction energy shown in Table 1. The analysis of the different contributions (see Table S3, ESI†) shows that the major difference between the proteins is in the interaction between Asp and the environment, while the FAD experiences a similar electrostatic potential.
To obtain further insight, we computed the contributions of the individual amino acid residues to ΔEcoul, visualized in the colouring scheme of Fig. 9 (see also Fig. S4 in the ESI†). The analysis shows three major factors being responsible for the energy difference: the different position of arginine 344/362 close to FAD, the interaction between Asp378 and Glu363 and a different interaction with water molecules.
No positive value of ΔEcoul larger than +0.3 kcal mol−1, and therefore disfavouring the FADH˙ state, was observed in CRYI. In contrast, in PL-N378D, several positive contributions stand out: +0.3, +0.4 and +2.9 kcal mol−1 for Leu375, Gly381 and Arg344, respectively. Thus, Arg344 (Arg362 in CRYI) interacts differently in PT PL-N378D: while it supports PT in CRYI (−1.74 kcal mol−1), it disfavours it in the PL mutant. The distance between Arg and FAD is on average shorter in PL-N378D (see the ESI,† Table S1), which could explain part of the preference for the negatively charged FAD˙− state.
Furthermore, in PL-N378D, Glu363 is strongly hydrogen-bonded to the negatively charged Asp378 (ΔEcoul = −10.32 kcal mol−1), while in CRYI, the homologous Met381 just slightly interacts with the FAD-Asp complex (ΔEcoul = −1.05 kcal mol−1). At first sight it may seem that this residue is not a good choice for stabilization of FADH˙. However, Met381 shows flexibility allowing water molecules to approach Asp396 resulting in a stabilizing interaction of −5.58 kcal mol−1 with negatively charged Asp. In contrast, the interaction with water molecules is positive (7.51 kcal mol−1) in the PL mutant, destabilizing the product state. We investigated the PL-N378D/E363M double mutant (see Fig. S5 in ESI†); however, no improved stabilization of the PT product was observed.
We also quantified the stabilization of FADH− induced by the pocket after the second photo-reduction. To this end, we calculated the energy of the HOMO of FADH˙− in WT-PL, PL-N378D and CRYI (further details are provided in the ESI†) during a short DFTB/MM calculation. The pocket of PL-WT induces a decrease of the orbital energy of 1.48 eV, i.e. 0.69 eV more than in CRYI (see Fig. S6 in the ESI†).
The protonation of the isoalloxazine ring occurs after its photo-reduction by means of a complex ET through a tryptophan triad. This first step occurs on a subnanosecond timescale, whereas the protonation step is at least four orders of magnitude slower: about 1.7 μs and 4 s in plant CRYI and E. coli PL respectively. Such a timescale difference and the experimental characterization of FAD˙− exclude a coupled electron-proton transfer mechanism (PCET). The environment has time to relax around FAD˙− after the fast photo-reduction. According to our MD simulations, the photo-reduction can lead to some structural rearrangements which consist of prerequisites to PT: the rotation of the PL-Asn378 or the CRYI-Asp396 side chain (close to FAD N5) or the entry of water molecules in the PL FAD pocket. Such observations corroborate the two step formation of the protonated semiquinone FADH˙: the photo-reduction triggers the conformational changes required for a PT, independently of the pH, and then, the basic FAD˙− is protonated.
We first identify a pathway to de/protonate FAD in E. coli PL, and then determine the energetics along this pathway. Unlike CRYI, PL has no close titratable residue that might provide a proton, so a more distant proton donor has to be sought, as has a proton transfer pathway connecting that donor to FAD. Free MD simulations and free energy calculations reveal that the Asn378 side chain plays an important role: its N-orientation is preferred with FAD˙−, and it does not allow for any protonation pathway to be formed, whereas the O-conformation is preferred in other states.62 Indeed, the N-conformation may be disfavoured by the steric hindrance between H–N5 of protonated FAD and the Asn378 side chain. Still, Asn378 may remain in the O-conformation for a certain time period after FAD˙− is formed, and we describe how a PT pathway can arise then: two water molecules may enter the FAD binding pocket at a moderate energy cost and these are sufficient to relay a proton from a proton donor like, e.g., the Glu106 side chain, or another external donor. The PT reaction along this pathway is even energetically favourable, meaning that the protonated FADH˙ is stabilized, with a strong basic character (pKa evaluated at 11.5). Asn378 can contribute to the stabilization of protonated FAD in PL by the formation of a hydrogen bond between the amido oxygen of Asn378 (in the O-conformation) and N5–H of FADH˙ and FADH− states, as reported before.62
In contrast, in CRYI, Asp396 works as a prolific proton relay and allows switching between protonated and deprotonated semiquinone FAD.28 In addition, we suppose that this residue, in its negative form, impairs the formation of a fully reduced FADH−. As expected, the presence of a close negatively charged Asp disfavours the second reduction of FAD compared to a neutral Asn. Then, we like to investigate whether Asp396/Asn378 is really the one residue that is the key to the different de/protonation mechanisms of CRY and PL. To answer this question and mimic previous experiments,20 we study the PL-N378D mutant, which unexpectedly disables the FAD protonation. Reversely, the single point mutation in CRYI-D396N stabilizes protonated FAD states and is able to repair DNA lesions.10
In contrast to our previous result in CRYI, the free energy profile of PT in the PL-N378D mutant shows that the deprotonated FAD˙− is favoured over FADH˙, in spite of the presence of the proton donor Asp378. The barrier opposing PT is quite low, allowing fast proton exchanges between the isoalloxazine ring and Asp. This result is consistent with the experimental multi-component UV-vis spectrum called FADx. The entirely different energetics of PT between CRYI and PL-N378D must have structural causes. A possible explanation comes to light as soon as the electrostatic potentials induced by the protein surroundings are analysed: the combined electrostatic effect of close amino acid residues and water molecules clearly favours the FADH˙–Asp378− state in CRYI, while it slightly stabilizes the reverse state in the PL mutant. Furthermore, a higher flexibility around FAD is observed in our MD simulations of CRYI, in agreement with previous experimental results.63,64
In the overall picture, it seems that the different protonation propensities of PL and CRYI are caused by multiple effects, based on both structural and dynamical contributions, with a large role played by water molecules transiently present around the FAD pocket. Despite the evident difference between the impacts of Asp and Asn on the favoured FAD redox state, a straightforward substitution of one or two isolated amino acids cannot modify PL to create the PT ability of CRYI in PL.
Footnote |
† Electronic supplementary information (ESI) available. See DOI: 10.1039/c9cp00694j |
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