Biomolecular NMR Assignments

, Volume 12, Issue 1, pp 79–83 | Cite as

1H, 15N and 13C backbone resonance assignments of pentaerythritol tetranitrate reductase from Enterobacter cloacae PB2

  • Andreea I. Iorgu
  • Nicola J. Baxter
  • Matthew J. Cliff
  • Jonathan P. Waltho
  • Sam Hay
  • Nigel S. Scrutton
Open Access
Article

Abstract

Pentaerythritol tetranitrate reductase (PETNR) is a flavoenzyme possessing a broad substrate specificity and is a member of the Old Yellow Enzyme family of oxidoreductases. As well as having high potential as an industrial biocatalyst, PETNR is an excellent model system for studying hydrogen transfer reactions. Mechanistic studies performed with PETNR using stopped-flow methods have shown that tunneling contributes towards hydride transfer from the NAD(P)H coenzyme to the flavin mononucleotide (FMN) cofactor and fast protein dynamics have been inferred to facilitate this catalytic step. Herein, we report the near-complete 1H, 15N and 13C backbone resonance assignments of PETNR in a stoichiometric complex with the FMN cofactor in its native oxidized form, which were obtained using heteronuclear multidimensional NMR spectroscopy. A total of 97% of all backbone resonances were assigned, with 333 out of a possible 344 residues assigned in the 1H–15N TROSY spectrum. This is the first report of an NMR structural study of a flavoenzyme from the Old Yellow Enzyme family and it lays the foundation for future investigations of functional dynamics in hydride transfer catalytic mechanism.

Keywords

Pentaerythritol tetranitrate reductase Flavoenzyme Flavin mononucleotide Backbone resonance assignment Transverse relaxation optimized spectroscopy 

Biological context

Pentaerythritol tetranitrate reductase (PETNR, EC 1.6.99.1) is a monomeric flavoenzyme that possesses a broad substrate specificity and is a member of the Old Yellow Enzyme (OYE) family of oxidoreductases (Toogood et al. 2010). PETNR was originally isolated from an Enterobacter cloacae PB2 strain that was thriving on soil contaminated with explosives by exploiting nitrate esters as metabolic nitrogen sources (French et al. 1996). The catalytic cycle of PETNR has been thoroughly investigated using stopped-flow techniques (Khan et al. 2002, 2005; Basran et al. 2003) and it is understood that the reaction chemistry takes place via a bi–bi ping–pong mechanism, with NADPH as the preferred coenzyme (NADH also supports catalysis, but in a less efficient manner). The first catalytic step, described as the reductive half-reaction, consists of the formation of a charge-transfer complex upon NAD(P)H binding, which enables subsequent hydride transfer from the nicotinamide ring C4 atom of NAD(P)H to the N5 atom of oxidized FMN (FMNox). The second step of the reaction, the oxidative half-reaction, is represented by hydride transfer from the N5 atom of reduced FMN to an α,β-unsaturated substrate and, in some cases, additional proton transfer from a solvent molecule. The specific biological role of PETNR is unknown, as for all members of the OYE family of oxidoreductases (Williams and Bruce 2002). However, whilst the biological substrate has yet to be discovered, many studies have unveiled the promiscuous nature of PETNR, as it catalyzes the reduction of a wide variety of α,β-unsaturated compounds, often with high specificity and enantioselectivity towards desired products (Toogood et al. 2011). PETNR acts as an ene-reductase, by reducing 2-cyclohexenone and several steroids to their corresponding alkanes, but also catalyzes the reduction of cyclic triazines, various explosives (e.g. pentaerythritol tetranitrate and trinitrotoluene) and nitrate esters (e.g. nitroglycerin). Several mutagenesis studies have highlighted the versatility of PETNR in the asymmetric reduction of C=C bonds, leading to an increased interest in understanding the physical basis of the catalytic power of this enzyme (Mueller et al. 2010; Fryszkowska et al. 2011; Toogood et al. 2011).

As well as having high potential to be used in biocatalytic processes, PETNR is an excellent model system for studying hydride transfer reactions. Previous kinetic studies have revealed that quantum mechanical tunneling contributes to the enzymatic hydride transfer step from NAD(P)H to the FMN cofactor, as the reaction manifests elevated kinetic isotope effects (Basran et al. 2003). Moreover, fast protein dynamics have been inferred to contribute to catalysis from various temperature and pressure dependence studies, coupled with the use of different isotopic labeling strategies (Pudney et al. 2009, 2013; Longbotham et al. 2016). However, the difference in reactivity of PETNR towards NADPH and NADH is still not clearly understood and the role of fast protein dynamics in catalytic events requires an atomistic description of the enzyme, as kinetic data alone cannot pinpoint or specifically isolate time-resolved structural changes. Herein, we report the near-complete, sequence-specific 1H, 15NH, 13Cα, 13Cβ and 13C′ backbone resonance assignments of PETNR in the PETNR:FMNox complex. The assignments provide a basis for further structural and functional studies by NMR spectroscopy, enabling more complex dynamic studies that can advance our understanding of enzymatic hydride transfer reactions.

Methods and experiments

All reagents were of analytical grade and were purchased from Sigma-Aldrich (UK), except for 15NH4Cl and 2H2O (> 99.9% purity), which were procured from Goss Scientific Ltd. (UK) and 2H7,13C6-d-glucose (> 98% purity), which was purchased from Cambridge Isotope Laboratories (USA).

Recombinant PETNR is expressed and purified as a tight non-covalently bound PETNR:FMNox complex. A pBlueScript II SK(+) plasmid encoding the pONR1 gene was used for PETNR overexpression. The 2H,13C,15N-labeled PETNR:FMNox complex (40 kDa) was expressed in JM109 E. coli cells grown in 100% 2H2O modified minimal media, using 15NH4Cl and 2H7,13C6-d-glucose as nitrogen and carbon sources, respectively. Cells were incubated at 37 °C with shaking at 200 rpm, until OD600nm = 0.8–1.0, after which the temperature was lowered to 25 °C and PETNR overexpression was induced by the addition of 0.5 mM isopropyl β-d-1-thiogalactopyranoside (IPTG). Cells were grown for a further 24 h before being harvested by centrifugation (6000 rpm for 15 min at 4 °C). All purification steps, which include affinity chromatography using a Mimetic Orange 2 column followed by Source 15Q anion exchange chromatography, were performed at 4 °C, as previously described (French et al. 1996; Barna et al. 2001). A final yield of approximately 70 mg pure PETNR per liter of cell culture was obtained.

Following purification, back exchange to amide protium atoms in the 2H,13C,15N-labeled PETNR:FMNox complex was promoted by mild destabilization using guanidine hydrochloride (GuHCl) as a denaturing agent, followed by rapid protein refolding. Partial unfolding of PETNR was initiated by mixing the sample (0.25 mM) in a 1:1 ratio with 1.5 M GuHCl solution in 50 mM potassium phosphate buffer (pH 7.0), followed by incubation at room temperature for 120 min. Refolding of PETNR was achieved by rapid 30-fold dilution into 50 mM potassium phosphate buffer (pH 7.0), under vigorous stirring. The resulting sample was filtered using a 0.2 μm filter-syringe to remove any precipitates, buffer-exchanged (to remove GuHCl) and concentrated using a Vivaspin 20 concentrator (10 kDa MWCO, Sigma-Aldrich, UK). The concentration of the PETNR:FMNox complex was estimated by measuring the FMN-specific absorbance peak at 464 nm (ε = 11.3 mM−1 cm−1).

All NMR experiments were conducted with samples containing 1 mM 2H,13C,15N-labeled PETNR:FMNox complex in 50 mM potassium phosphate buffer (pH 7.0) supplemented with 1 mM NaN3, 10% (v/v) 2H2O for the deuterium lock and 0.5% (v/v) trimethylsilyl propanoic acid (TSP) for chemical shift referencing. The samples (300 μL) were centrifuged for 10 min at 13,000 rpm before being transferred to 5-mm Shigemi tubes (Sigma-Aldrich, UK). All NMR experiments were recorded at 298 K on an 800 MHz Bruker Avance III spectrometer running TopSpin version 3.2, equipped with a 5-mm 1H/13C/15N TCI cryoprobe and a Z-field gradient coil. The backbone resonance assignment of PETNR was achieved using standard Bruker 1H–15N TROSY and TROSY-based 3D HNCA, HNCACB, HN(CO)CACB, HN(CA)CO and HNCO triple resonance experiments (Gardner and Kay 1998). The 3D experiments were acquired using non-uniform sampling with a sine-weighted multidimensional Poisson Gap scheduling strategy (Hyberts et al. 2013). 1H chemical shifts were referenced relative to the internal TSP signal, whereas 15N and 13C chemical shifts were referenced indirectly using nuclei-specific gyromagnetic ratios (Markley et al. 1998). NMR data were processed using TopSpin software version 3.2 and analyzed using CcpNmr Analysis software version 2.4 (Vranken et al. 2005).

Resonance assignment and data deposition

Using conventional TROSY-based 3D heteronuclear experiments, sequential backbone assignment of PETNR in the PETNR:FMNox complex was achieved to a great extent, with 97% of backbone amide groups successfully assigned (333 out of 344 non-proline residues) in the 1H–15N TROSY spectrum (Fig. 1). A similar degree of assignment (97%) was achieved for the corresponding 13Cα, 13Cβ and 13C′ resonances: 354 out of all 364 Cα atoms, 320 out of all 330 Cβ atoms and 354 out of all 364 C′ atoms. The chemical shift assignments have been deposited in the Biological Magnetic Resonance Bank (BMRB: http://www.bmrb.wisc.edu/) under the accession number 27224.

Fig. 1

1H–15N TROSY spectrum of 1 mM uniformly 2H,13C,15N-labeled PETNR:FMNox complex in 50 mM potassium phosphate buffer (pH 7.0), recorded at 298 K on an 800 MHz spectrometer. The full spectrum (a) and two expansions of the crowded regions (b) are shown. The assignment of the backbone amide resonances are indicated by sequence number and residue type

The assignment extends the list of large molecular systems that have undergone essentially complete backbone assignment, at a time where limits are being pushed with studies of very large biological systems (Sprangers and Kay 2007). The assignment of PETNR was facilitated by the wide dispersion and favorable line shape of the resonances in the 1H–15N TROSY spectrum, attributed to the globular folded structure, isotopic labeling strategy and correlation time of the complex (21 ns). There are ten residues that remain unassigned in the 1H–15N TROSY spectrum (A2, G34, G115, H184, S206, E272, T273, D274, L275 and A276), which are mainly located in a mobile loop (E272–Y281), at the N-terminus and in other solvent-exposed regions of PETNR (Fig. 2). The E272–Y281 loop is located at the edge of the substrate-binding pocket of the active site, but is solvent exposed in the PETNR:FMNox complex and residues T273–A284 have high temperature factors and limited secondary structure, as it has been observed from crystallographic data (Barna et al. 2001). Thus, both conformational exchange and solvent exchange are probably the source of signal attenuation beyond detection in the 1H–15N TROSY spectrum for residues E272, T273, D274, L275 and A276. Residue A2, located at the N-terminus, and residues G34, G115 and S206, located at the surface of PETNR, could not be assigned since their 1H–15N TROSY correlations are likely attenuated due to fast exchange with solvent. Residue H184 is known to be involved in substrate coordination (Barna et al. 2001) and, in the absence of bound substrate, will probably be undergoing conformational exchange on the millisecond timescale.

Fig. 2

Cartoon representation of the crystal structure of the PETNR:FMNox complex [PDB: 5LGX (Kwon et al. 2017)], highlighting the extent of backbone amide resonance assignments. Assigned residues are colored light orange (for α-helices and loops) and pale green (for β-strands), with unassigned residues shown in red and proline residues in purple. The non-covalently bound FMN cofactor is depicted as yellow sticks

An empirical prediction of the secondary structure elements of PETNR in the PETNR:FMNox complex was performed by uploading the backbone 1HN, 15N, 13Cα, 13Cβ and 13C′ chemical shift assignments to the TALOS-N webserver (Shen and Bax 2013). The results of the prediction are illustrated in Fig. 3, along with a comparison of the secondary structure present in the crystal form of the complex. The prediction derived from the NMR data is in very good agreement with the crystallographic data, with all the specific elements of the eight-stranded α/β barrel (TIM barrel) predicted accurately. The results provide high confidence in the assignments of the PETNR:FMNox complex.

Fig. 3

Backbone secondary structure prediction of PETNR in the PETNR:FMNox complex obtained with TALOS-N software (Shen and Bax 2013) using the backbone 1HN, 15N, 13Cα 13Cβ and 13C′ chemical shifts. The secondary structure prediction is depicted as red bars and blue bars for α-helices and β-strands, respectively, with the height of the bars reflecting the probability of each element, as assigned by the software. As a comparison, the secondary structure observed in the crystal form of the PETNR:FMNox complex [PDB: 5LGX (Kwon et al. 2017)] is shown at the top of the figure in the same color representation

Notes

Acknowledgements

A.I.I. is an Early Stage Researcher supported by the EU’s Seventh Framework Programme through the Marie Curie Initial Training Network MAGIC (Grant Agreement No. 606831). N.J.B. is supported by the Biotechnology and Biological Sciences Research Council (BBSRC) (BB/M021637/1). N.S.S. is an Engineering and Physical Sciences Research Council (EPSRC) Established Career Fellow (EP/J020192/1).

References

  1. Barna TM, Khan H, Bruce NC et al (2001) Crystal structure of pentaerythritol tetranitrate reductase: “flipped” binding geometries for steroid substrates in different redox states of the enzyme. J Mol Biol 310:433–447. doi: 10.1006/jmbi.2001.4779 CrossRefGoogle Scholar
  2. Basran J, Harris RJ, Sutcliffe MJ, Scrutton NS (2003) H-tunneling in the multiple H-transfers of the catalytic cycle of morphinone reductase and in the reductive half-reaction of the homologous pentaerythritol tetranitrate reductase. J Biol Chem 278:43973–43982. doi: 10.1074/jbc.M305983200 CrossRefGoogle Scholar
  3. French CE, Nicklin S, Bruce NC (1996) Sequence and properties of pentaerythritol tetranitrate reductase from Enterobacter cloacae PB2. J Bacteriol 178:6623–6627. doi: 10.1128/jb.178.22.6623-6627.1996 CrossRefGoogle Scholar
  4. Fryszkowska A, Toogood H, Sakuma M et al (2011) Active site modifications in pentaerythritol tetranitrate reductase can lead to improved product enantiopurity, decreased by-product formation and altered stereochemical outcome in reactions with α,β-unsaturated nitroolefins. Catal Sci Technol 1:948–957. doi: 10.1039/c0cy00092b CrossRefGoogle Scholar
  5. Gardner KH, Kay LE (1998) The use of 2H, 13C, 15N multidimensional NMR to study the structure and dynamics of proteins. Annu Rev Biophys Biomol Struct 27:357–406. doi: 10.1146/annurev.biophys.27.1.357 CrossRefGoogle Scholar
  6. Hyberts SG, Robson SA, Wagner G (2013) Exploring signal-to-noise ratio and sensitivity in non-uniformly sampled multi-dimensional NMR spectra. J Biomol NMR 55:167–178. doi: 10.1007/s10858-012-9698-2 CrossRefGoogle Scholar
  7. Khan H, Harris RJ, Barna T et al (2002) Kinetic and structural basis of reactivity of pentaerythritol tetranitrate reductase with NADPH, 2-cyclohexenone, nitroesters, and nitroaromatic explosives. J Biol Chem 277:21906–21912. doi: 10.1074/jbc.M200637200 CrossRefGoogle Scholar
  8. Khan H, Barna T, Bruce NC et al (2005) Proton transfer in the oxidative half-reaction of pentaerythritol tetranitrate reductase. Structure of the reduced enzyme-progesterone complex and the roles of residues Tyr186, His181, His184. FEBS J 272:4660–4671. doi: 10.1111/j.1742-4658.2005.04875.x CrossRefGoogle Scholar
  9. Kwon H, Smith O, Raven EL, Moody PCE (2017) Combining X-ray and neutron crystallography with spectroscopy. Acta Crystallogr D 73:141–147. doi: 10.1107/S2059798316016314 CrossRefGoogle Scholar
  10. Longbotham JE, Hardman SJO, Görlich S et al (2016) Untangling heavy protein and cofactor isotope effects on enzyme-catalyzed hydride transfer. J Am Chem Soc 138:13693–13699. doi: 10.1021/jacs.6b07852 CrossRefGoogle Scholar
  11. Markley JL, Bax A, Arata Y et al (1998) Recommendations for the presentation of NMR structures of proteins and nucleic acids—IUPAC-IUBMB-IUPAB Inter-Union Task Group on the standardization of data bases of protein and nucleic acid structures determined by NMR spectroscopy. J Biomol NMR 12:1–23. doi: 10.1023/A:1008290618449 CrossRefGoogle Scholar
  12. Mueller NJ, Stueckler C, Hauer B et al (2010) The substrate spectra of pentaerythritol tetranitrate reductase, morphinone reductase, N-ethylmaleimide reductase and estrogen-binding protein in the asymmetric bioreduction of activated alkenes. Adv Synth Catal 352:387–394. doi: 10.1002/adsc.200900832 CrossRefGoogle Scholar
  13. Pudney CR, Hay S, Levy C et al (2009) Evidence to support the hypothesis that promoting vibrations enhance the rate of an enzyme catalyzed H-tunneling reaction. J Am Chem Soc 131:17072–17073. doi: 10.1021/ja908469m CrossRefGoogle Scholar
  14. Pudney CR, Guerriero A, Baxter NJ et al (2013) Fast protein motions are coupled to enzyme H-transfer reactions. J Am Chem Soc 135:2512–2517. doi: 10.1021/ja311277k CrossRefGoogle Scholar
  15. Shen Y, Bax A (2013) Protein backbone and sidechain torsion angles predicted from NMR chemical shifts using artificial neural networks. J Biomol NMR 56:227–241. doi: 10.1007/s10858-013-9741-y CrossRefGoogle Scholar
  16. Sprangers R, Kay LE (2007) Quantitative dynamics and binding studies of the 20S proteasome by NMR. Nature 445:618–622. doi: 10.1038/nature05512 CrossRefGoogle Scholar
  17. Toogood HS, Gardiner JM, Scrutton NS (2010) Biocatalytic reductions and chemical versatility of the Old Yellow Enzyme family of flavoprotein oxidoreductases. ChemCatChem 2:892–914. doi: 10.1002/cctc.201000094 CrossRefGoogle Scholar
  18. Toogood HS, Fryszkowska A, Hulley M et al (2011) A site-saturated mutagenesis study of pentaerythritol tetranitrate reductase reveals that residues 181 and 184 influence ligand binding, stereochemistry and reactivity. ChemBioChem 12:738–749. doi: 10.1002/cbic.201000662 CrossRefGoogle Scholar
  19. Vranken WF, Boucher W, Stevens TJ et al (2005) The CCPN data model for NMR spectroscopy: development of a software pipeline. Proteins 59:687–696. doi: 10.1002/prot.20449 CrossRefGoogle Scholar
  20. Williams RE, Bruce NC (2002) “New uses for an Old Enzyme”—the Old Yellow Enzyme family of flavoenzymes. Microbiology 148:1607–1614. doi: 10.1099/00221287-148-6-1607 CrossRefGoogle Scholar

Copyright information

© The Author(s) 2017

Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made.

Authors and Affiliations

  1. 1.Manchester Institute of Biotechnology and School of ChemistryThe University of ManchesterManchesterUK
  2. 2.Krebs Institute for Biomolecular Research, Department of Molecular Biology and BiotechnologyThe University of Sheffield, Firth Court, Western BankSheffieldUK

Personalised recommendations