Biomolecular NMR Assignments

, Volume 13, Issue 1, pp 187–193 | Cite as

Complete NMR chemical shift assignments of odorant binding protein 22 from the yellow fever mosquito, Aedes aegypti, bound to arachidonic acid

  • David N. M. JonesEmail author
  • Jing Wang
  • Emma J. Murphy
Open Access


Aedes aegypti mosquitoes are the vector for transmission of Dengue, Zika and chikungunya viruses. These mosquitos feed exclusively on human hosts for a blood meal. Previous studies have established that Dengue virus infection of the mosquito results in increased expression of the odorant binding proteins 22 and 10 within the mosquito salivary gland and silencing of these genes dramatically reduces blood-feeding behaviors. Odorant binding proteins are implicated in modulating the chemosensory perception of external stimuli that regulate behaviors such as host location, feeding and reproduction. However, the role that AeOBP22 plays in the salivary gland is unclear. Here, as a first step to a more complete understanding of the function of AeOBP22, we present the complete backbone and side chain chemical shift assignments of the protein in the complex it forms with arachidonic acid. These assignments reveal that the protein consists of seven α-helices, and that the arachidonic acid is bound tightly to the protein. Comparison with the chemical shift assignments of the apo-form of the protein reveals that binding of the fatty acid is accompanied by a large conformational change in the C-terminal helix, which appears disordered in the absence of lipid. This NMR data provides the basis for determining the structure of AeOBP22 and understanding the nature of the conformational changes that occur upon ligand binding. This information will provide a path to discover novel compounds that can interfere with AeOBP22 function and impact blood feeding by this mosquito.


Aedes aegypti Odorant binding protein 22 Arachidonic acid NMR resonance assignments 

Biological context

Aedes aegypti mosquitoes are responsible for the transmission of multiple diseases that including Dengue, chikungunya, Zika and yellow fever viruses. Whilst these diseases have been considered largely tropical in nature, the impact of climate change has dramatically increased the potential ranges for these mosquitoes into densely populated areas within the US and elsewhere. Disease transmission occurs when a female mosquito takes a blood meal from a human host. Aedes aegypti, in common with the malaria mosquito Anopheles gambiae, has evolved to feed exclusively on humans and this host selection is regulated by the perception of specific chemical cues that emanate from the human hosts (Braks et al. 1999). The presence of different chemical signatures directly impacts the attractiveness of an individual to the mosquito (Verhulst et al. 2013). It has been shown that mosquitoes infected with the malaria parasite Plasmodium falciparum exhibit increased attraction to human scent (Smallegange et al. 2013). Whilst humans infected with the parasite, are more attractive to mosquitoes (Lacroix et al. 2005).

Recently, it was shown that Dengue virus infection of Ae. aegypti could also potentially impact control of mosquito feeding behaviors (Sim et al. 2012). Viral infection was found to increase the expression of a set of chemosensory genes within the mosquito salivary gland, which included the odorant binding proteins (OBPs) 22 and 10 (AeOBP22 and AeOBP10) (Sim et al. 2012). Subsequently, it was demonstrated that knock down of these genes using siRNA approaches led to a significant reduction in the blood feeding behavior of these mosquitoes (Sim et al. 2012).

Odorant binding proteins are a highly abundant and diverse group of proteins (Hekmat-Scafe et al. 2002) that are generally found in the chemosensory tissues of insects (Shanbhag et al. 2001) where they can bind to a range of chemically related ligands(Campanacci et al. 2001; Honson et al. 2003; Pelosi et al. 2006; Plettner et al. 2000; Swarup et al. 2011). There is evidence for multiple roles of OBPs, including transporting ligands to the vicinity of odorant receptors (Damberger et al. 2000; Horst et al. 2001; Sandler et al. 2000; Wojtasek and Leal 1999; Ziegelberger 1995), activating odorant receptor complexes (Berg and Ziegelberger 1991; Laughlin et al. 2008; Pophof 2002, 2004; Xu et al. 2005), modulating sensitivity of odorant receptors (Larter et al. 2016) and terminating signal transmission (Vogt and Riddiford 1981; Ziegelberger 1995). AeOBP22 is expressed in multiple tissues, including the antenna, the salivary gland, the male reproductive tissues, and is transferred to females during mating (Li et al. 2008; Sim et al. 2012), suggesting that this OBP may regulate multiple behaviors that range from host seeking and feeding to reproduction. Therefore AeOBP22 is a novel target to potentially disrupt transmission of Ae. aegypti borne infections and also control of mosquito populations.

Preliminary screens of potential ligands have revealed compounds that can bind to AeOBP22 in the high nanomolar to micromolar range (Li et al. 2008; Yang et al. 2011). However, there is no data that links these binding events to any changes in mosquito behavior. In order to better define the specific compounds that AeOBP22 can bind, and how this binding may regulate blood feeding, we have initiated structural and biochemical studies of the protein. In the process we discovered that AeOBP22 binds very tightly to lipids and fatty acids. Here, we present the backbone and side chain chemical shift assignments of AeOBP22 in the complex that it forms with arachidonic acid (AA). These results represent the first reported NMR chemical shift assignments of arachidonic acid in a complex with a protein, and only the second ever NMR solution based studies of a protein-arachidonic acid complex (Coudevylle et al. 2011). We show that AeOBPP22 binds arachidonic acid in a tight, stable complex, and we identify the region of the protein that undergoes a significant conformational change upon binding ligand. We propose that this conformational change regulates ligand binding and release, and a complete structural analysis will allow for the discovery of novel ligands that can disrupt ligand binding.

Materials and methods

Protein expression and purification

The majority of odorant binding proteins in insects are secreted proteins, and analysis of the Ae. aegypti OBP22 gene (Vector base AAEL005772) using the Signal-IP v 4.1 (Petersen et al. 2011) predicts a cleavage site for the signal peptide between residues 16 and 17 of the full length protein. We used Ae. aegypti cDNA (gift from Dr. Richard Vogt) to PCR amplify and subclone the gene fragment corresponding to the mature form of the protein ( residues 17–138) into the NdeI and BamH1 restrictions site of the pET13a vector (Studier et al. 1990). This construct lacks the native signal peptide sequence but introduces an N-terminal initiator methionine; otherwise the vector contains no expression tags. We have numbered our assignments with the methionine considered as residue 1. The protein was expressed in Escherichia coli BL21(DE3) in cell cultures grown in minimal media supplemented with 2 g/L 13C D-glucose (> 99 atom %) and 1 g/L 15N NH4Cl (> 98 atom %) (Sigma Aldrich). Cells were grown at 37 °C to an OD600 of 0.5–0.6, and protein expression induced by addition of 1 mM isopropyl-1-thio-d-galactopyranoside (IPTG) and grown with shaking overnight at 25 ºC. The protein expressed in this way was purified from inclusion bodies essentially as previously described (Kruse et al. 2003; Murphy et al. 2013). The published protocol was modified in that the crude inclusion body pellet was washed three times with wash buffer 1 (20 mM Tris, pH 7.5, 0.5% Triton X-100, 1 mM EDTA and 1M Urea) followed by three times with wash buffer 2 (20 mM Tris, pH 7.5, 1 mM EDTA). The pellets were sonicated for 2 × 30 s during each wash step. The washed pellet was solubilized in 5 M guanidine hydrochloride, 5 mM dithiothreitol and 0.5 mM PMSF and the denatured protein was refolded using a cysteine/cystine redox reaction in the presence of 1% butanol, as previously described (Kruse et al. 2003; Murphy et al. 2013). The resulting protein solution was extensively dialyzed against sodium phosphate buffer (20 mM, pH 6.5), concentrated, and purified using size exclusion chromatography (Superdex S75) on an AKTA purifier system (Amersham Pharmicia Biotech). Purified protein, which eluted as a monomer, was checked for correct folding by circular dichroism (CD) spectroscopy (15 µM and at 25 °C) on a Jasco-815 spectropolarimeter in the CU School of Medicine biophysics core.

Samples of the complex between AeOBP22 and arachidonic acid (NuCheck Prep, Elysian MN) were made by addition of the arachidonic acid (in ethanol) to a final concentration of 200 µM to a sample of the protein at a concentration of 100 µM, and this was incubated overnight at 25 °C, concentrated and the buffer exchanged 3x to remove excess ethanol.

NMR experiments

NMR experiments were recorded using 15N and 13C labeled protein (400–650 µM) in 20 mM sodium phosphate at pH 6.5, 10% D2O and 2,2,-dimethyl-2-silapentane-5-sulfonic acid (DSS) (80 μM) as the internal chemical shift reference. NMR experiments were performed at 25 °C on a Varian INOVA 600 MHz or a Varian/Agilent DD2 900 MHz spectrometer both equipped with cryoprobes. Assignments of the protein main-chain atoms were made using sensitivity enhanced versions of 2D 1H/15N-HSQC and 2D 1H/13C-HSQC (Kay et al. 1992), 3D HNCO (Grzesiek and Bax 1992b; Muhandiram and Kay 1994), 3D (HACA)CO(CA)NH (Lohr and Ruterjans 1995), 3D HNCACB and CBCA(CO)NH (Grzesiek and Bax 1992a), 3D CC(CO)NH (Grzesiek et al. 1993). While assignments of side chain 13C and 1H resonances were made using 3D HBHA(CBCACO)NH (Grzesiek and Bax 1993), 3D H(CCCO)NH (Grzesiek et al. 1993) and a simultaneous 3D 15N/13C- NOESY-HSQC (Vögeli et al. 2013). This latter experiment was modified from the published version to use broadband adiabatic inversion pulses on 13C during the INEPT periods. Aromatic protons were assigned from 2D (HB)CB(CGCD)HD and (HB)CB(CGCDCE)HE experiments (Yamazaki et al. 1993).

All 3D experiments were collected using non uniform sampling methods (Barna et al. 1987) using the Poisson-gap sampling schemes implemented by Hyberts et al. (Hyberts et al. 2010) and with a sampling density of 25–40%. Sampling densities were generally selected based on the expected dynamic range, with lower sampling densities being used in experiments with higher signal to noise and more uniform peak intensities, e.g. HNCO and CBCA(CO)NH where reconstruction artifacts were less likely to impact data interpretation, whilst NOESY spectra were acquired with the highest sampling densities. Data were processed using the istHMS package v2111 (Hyberts et al. 2014, 2012) in combination with NMRpipe (Delaglio et al. 1995) and resonance assignments were determined using Ccpnmr Analysis v 2.4.2 (Vranken et al. 2005).

The assignments of the arachidonic acid in the complex were made using 2D 15N/13C-filtered NOESY and TOCSY experiments (Ikura and Bax 1992; Zwahlen et al. 1997) (Fig. 2) recorded using a sample of the complex prepared in the same way but using 99% D2O containing sodium phosphate (20 mM, pH 6.1).

Extent of the assignments for the OBP22-archidonic acid complex

The assignments of OBP22 in the complex with arachidonic acid were made manually within Ccpnmr’s Analysis program. (Vranken et al. 2005). In the 1H-15N HSQC experiment the assignments of the backbone amides are 100% complete, with the exception of the N-terminal methionine (Fig. 1). In addition, assignments for the Cα, Cβ, Hα and Hβ resonances are also 100% complete. The backbone CO assignments are 96% complete, 4 assignments could not be made unambiguously because of overlap. Assignments of the Hγ and Cγ resonances, excluding CγO and Cγ of aromatic residues, are also 100% complete. 95% of the Cδ resonances could be assigned (excludes CδO, and Cδ in Trp). The three missing assignments are the Cδ of Phe32 and Phe57, which are overlapped with other aromatic resonances, and Lys48, which is line broadened due to conformational exchange. The Hε and Cε resonances are 73% and 75% complete respectively. Here the notable absences are the Hε1 protons of the three histidines, which all exhibit significant line broadening, that prevents unambiguous assignment. Finally the HZ and HH resonances are 83 and 100% assigned respectively. Analysis of the chemical shift assignments, confirms that AeOBP22 is predominantly α-helical, in common with other insect OBPs (Fig. 3).

Fig. 1

Backbone amide resonance assignment of AeOBP22 bound to arachidonic acid. The 2D [1H-15N] –HSQC spectrum of uniformly 13C/15N - labeled AeOBP22 recorded at 25 °C and at 900 MHz is shown and the peaks are labeled with the assignments. 100% of the non-proline residues could be assigned in this spectrum. Assignments of the side-chain NH2 groups from the Asn and Gln resides are indicated with an asterisk, and the pairs of protons are connected by dashed lines

Assignment of arachidonic acid

Only a single set of peaks are observed for the arachidonic acid resonances in the complex with OBP22. Further, the chemical shifts of the vinylic protons have significantly greater dispersion compared those observed in solution for the free fatty acid. 1H-15N-HSQC spectra recorded of the protein recorded using sub-stoichiometric concentrations of the lipid show two distinct sets of peaks (not shown), and these overlap with the peaks in the spectra of the free and bound states of the protein. Spectra recorded with increasing lipid concentration show a shift in the population of the peaks from the bound state and a reduction in the peaks from the free state, indicating that binding of the lipid is in slow exchange on the NMR timescale. This is in agreement with preliminary fluorescent based binding assays that suggest that arachidonic acid binds with a KD of ~ 230 nM. We interpret the lack of any signal from the free state of the lipid in the samples used for our NMR assignment and structure determination as a result of micelle formation as the critical micelle concentration for arachidonic acid is reported to be in the range 10–60 µΜ (Pompeia et al. 2003; Serth et al. 1991).

The assignment of the arachidonic acid proton resonances was facilitated by the virtue that each vinylic proton was in a unique environment within the protein and these resonances show limited overlap with resonances from the protein. An overlay of the 13C-filtered NOESY and TOCSY experiments showing the vinylic proton resonances from the lipid in the region between 4.8 and 6.0 ppm is shown in Fig. 2. A single proton at 5.625 ppm exhibits correlations to multiple methylene protons in the range 0.8–1.7 ppm, establishing it as originating from H15. Two other vinylic protons, at ~ 5.0 and 5.12 ppm show correlations to methylene protons in the range 1.3–2.0 ppm including to the H2 position (immediately adjacent to the C1 carboxyl group), establishing these as the H5 and H6 protons respectively. Using these as the entry points it was possible to assign all the remaining protons in the lipid chain. That all the protons in the lipid chain have unique chemical shifts, reflects the unique interactions that must be formed with the protein. Insect OBPs generally bind to ligands within a central binding cavity, and intermolecular NOESY experiments confirm that the arachidonic acid is binding in the central pocket of OBP22.

Fig. 2

Resonance assignments of arachidonic acid bound to AeOBP22. Overlay of the vinylic proton region from the 2D-[13C/15N]-filtered TOCSY (black) and NOESY (red) spectra recorded using uniformly 13C/15N—labeled AeOBP22 and unlabeled fatty acid. The spectrum suppresses signals from the protein. The vinylic protons at each end of the double bond (labels at bottom) exhibit characteristic correlations to the remaining protons within the lipid chain (labeled vertically at left), enabling facile assignment for the lipid

Backbone assignments of apo AeOBP22

In order to better understand the nature of any conformational changes that occur on ligand binding to AeOBP22 we also obtained backbone assignments for the H, N, Cα and Cβ resonances of the apo form of the protein. We have obtained assignments for 117 of the expected 119 amides for this sample. In the 1H-15N-HSQC spectrum of the apo protein we do not observe peaks for residues 2 and 116. There are large chemical shift differences between the apo and bound states of AeOBP22 in multiple locations in the protein, with the largest differences localized to the C-terminal residues 104–123 (Fig. 3a). A comparison of the calculated secondary structure propensities for the apo and bound states (Marsh et al. 2006) (Fig. 3b) reveals that the overall secondary structure of the protein is maintained throughout most of the protein between the apo and bound states. In contrast, the C-terminal residues are significantly less ordered in the apo state. This indicates that the binding of arachidonic acid may be regulated by a conformational change that occurs in the C-terminal region of the protein.

Fig. 3

The C-terminal tail of AeOBP22 undergoes a conformational change on binding lipid. a Plot of the normalized chemical shift difference between AeOBP22 in the apo state and bound to arachidonic acid as a function of residue number. Normalized shift differences were calculated as Δδ = sqrt (ΔδH2 + 0.15*ΔδN2). Residues that show shift changes greater than the mean are colored orange and those that are greater than 1 s.d. above the mean are colored red. Horizontal dashed lines indicated the values for the mean shift change and the mean plus 1 s.d. b Plot of the secondary structure propensity calculated using SSP (Marsh et al. 2006) for the apo AeOBP22 (red) and arachidonic acid bound protein (blue). The location of the predicted alpha-helical regions in the bound state is shown in the panel above as blue bars. For the apo-protein there is a clear break in the predicted secondary structure at residue 111


Aedes aegypti OBP22 is implicated in regulating the blood feeding behavior of this mosquito (Sim et al. 2012). However, the specific chemosensory stimulus(i) that is involved in this response is as yet unknown. In the process of trying to identify the natural ligands for AeOBP22, we have discovered that it binds tightly to fatty acids, including arachidonic acid. Here we have shown that the binding of arachidonic acid induces a significant conformational change in the C-terminal residues, suggesting that region of the protein may be responsible for regulating ligand binding. Further it is apparent that the arachidonic acid must adopt a highly defined conformation within the protein, as there is no evidence of chemical exchange for the lipid resonances. The question that arises is what functional role does AeOBP22 fulfill in binding arachidonic acid and/or other fatty acids. One hypothesis is that is recognizing specific lipids and delivering these to chemosensory receptors in the mosquito that are required to stimulate blood feeding. This would correlate with the observed reduction in feeding behaviors seen in dsRNA knock down of OBP22 gene expression (Sim et al. 2012). However, many fatty acids, including AA, are released from cell membranes by the activity of phospholipase A2. These can function both as intracellular messengers but also, as in the case of AA, as precursors of proinflammatory signals. Therefore, an alternative hypothesis is that AeOBP22 sequesters pro inflammatory signals as a mechanism to guard against premature termination of blood feeding.

Ongoing structural studies of AeOBP22 using the data presented here, will inform on the specific ligands that can interact with AeOBP22 and better inform on its biological function. Knowledge of the nature and magnitude of the conformational changes that take place when ligands bind will generate structural information that can used to discover novel compounds that have the potential to complete for ligand binding, disrupt OBP22 function, and impact the blood-feeding behavior of the mosquito.



This work was supported by NIH/NIAID Grant RO1 AI121253 to DNMJ. The operation of the NMR facilities at CU School of Medicine is supported in part by the University of Colorado Cancer Center Support Grant (NIH 5P30-CA046934).

Accession numbers

The chemical shift assignments for the AeOBP22-AA complex (BMRB 30550) and apo-AeOBP22 (BMRB 27724) have been deposited within the Biological Magnetic Resonance Data Bank.

Compliance with ethical standards

Conflict of interest

The authors declare they have no conflict of interest.


  1. Barna JCJ, Laue ED, Mayger MR, Skilling J, Worrall SJP (1987) Exponential sampling, an alternative method for sampling in two-dimensional NMR experiments. J Magn Reson 73:69–77. ADSGoogle Scholar
  2. Berg MJVD, Ziegelberger G (1991) On the function of the pheromone binding protein in the olfactory hairs of Antheraea polyphemus. J Insect Physiol 37:79–85CrossRefGoogle Scholar
  3. Braks MA, Anderson RA, Knols BG (1999) Infochemicals in mosquito host selection: human skin microflora and Plasmodium parasites. Parasitol Today 15:409–413CrossRefGoogle Scholar
  4. Campanacci V et al (2001) Revisiting the specificity of Mamestra brassicae and Antheraea polyphemus pheromone-binding proteins with a fluorescence binding assay. J Biol Chem 276:20078–20084CrossRefGoogle Scholar
  5. Coudevylle N, Hoetzinger M, Geist L, Kontaxis G, Hartl M, Bister K, Konrat R (2011) Lipocalin Q83 reveals a dual ligand binding mode with potential implications for the functions of siderocalins. Biochemistry 50:9192–9199. CrossRefGoogle Scholar
  6. Damberger F, Nikonova L, Horst R, Peng G, Leal WS, Wüthrich K (2000) NMR characterization of a pH-dependent equilibrium between two folded solution conformations of the pheromone-binding protein from Bombyx mori. Protein Sci 9:1038–1041. CrossRefGoogle Scholar
  7. Delaglio F, Grzesiek S, Vuister GW, Zhu G, Pfeifer J, Bax A (1995) NMRPipe: a multidimensional spectral processing system based on UNIX pipes. J Biomol NMR 6:277–293CrossRefGoogle Scholar
  8. Grzesiek S, Bax A (1992a) Correlating backbone amide and side chain resonances in larger proteins by multiple relayed triple resonance. NMR J Am Chem Soc 114:6291–6293. CrossRefGoogle Scholar
  9. Grzesiek S, Bax A (1992b) Improved 3D triple-resonance NMR techniques applied to a 31-KDa protein. J Magn Reson 96:432–440. ADSGoogle Scholar
  10. Grzesiek S, Bax A (1993) Amino acid type determination in the sequential assignment procedure of uniformly 13C/15N-enriched proteins. J Biomol NMR 3:185–204. Google Scholar
  11. Grzesiek S, Anglister J, Bax A (1993) Correlation of backbone amide and aliphatic side-chain resonances in C-13/N-15-enriched proteins by isotropic mixing of C-13 magnetization. J Magn Reson Ser B 101:114–119. CrossRefGoogle Scholar
  12. Hekmat-Scafe DS, Scafe CR, McKinney AJ, Tanouye MA (2002) Genome-wide analysis of the odorant-binding protein gene family in Drosophila melanogaster. Genome Res 12:1357–1369CrossRefGoogle Scholar
  13. Honson N, Johnson MA, Oliver JE, Prestwich GD, Plettner E (2003) Structure-activity studies with pheromone-binding proteins of the Gypsy Moth Lymantria dispar. Chem Senses 28:479–489CrossRefGoogle Scholar
  14. Horst R et al (2001) NMR structure reveals intramolecular regulation mechanism for pheromone binding and release. Proc Natl Acad Sci USA 98:14374–14379ADSCrossRefGoogle Scholar
  15. Hyberts SG, Takeuchi K, Wagner G (2010) Poisson-gap sampling and forward maximum entropy reconstruction for enhancing the resolution and sensitivity of protein NMR data. J Am Chem Soc 132:2145–2147. CrossRefGoogle Scholar
  16. Hyberts SG, Milbradt AG, Wagner AB, Arthanari H, Wagner G (2012) Application of iterative soft thresholding for fast reconstruction of NMR data non-uniformly sampled with multidimensional Poisson Gap scheduling. J Biomol NMR 52:315–327. CrossRefGoogle Scholar
  17. Hyberts SG, Arthanari H, Robson SA, Wagner G (2014) Perspectives in magnetic resonance: NMR in the post-FFT era. J Magn Reson 241:60–73. ADSCrossRefGoogle Scholar
  18. Ikura M, Bax A (1992) Isotope-filtered 2D NMR of a protein peptide complex: study of a skeletal-muscle myosin light chain kinase fragment bound to calmodulin. J Am Chem Soc 114:2433–2440. CrossRefGoogle Scholar
  19. Kay LE, Keifer P, Saarinen T (1992) Pure absorption gradient enhanced heteronuclear single quantum correlation spectroscopy with improved sensitivity. J Am Chem Soc 114:10663–10665. CrossRefGoogle Scholar
  20. Kruse SW, Zhao R, Smith DP, Jones DN (2003) Structure of a specific alcohol-binding site defined by the odorant binding protein LUSH from Drosophila melanogaster. Nat Struct Biol 10:694–700. CrossRefGoogle Scholar
  21. Lacroix R, Mukabana WR, Gouagna LC, Koella JC (2005) Malaria infection increases attractiveness of humans to mosquitoes. PLoS Biol 3:e298. CrossRefGoogle Scholar
  22. Larter NK, Sun JS, Carlson JR (2016) Organization and function of Drosophila odorant binding proteins. eLife 5.
  23. Laughlin JD, Ha TS, Jones DN, Smith DP (2008) Activation of pheromone-sensitive neurons is mediated by conformational activation of pheromone-binding protein Cell 133:1255–1265. CrossRefGoogle Scholar
  24. Li S, Picimbon J-F, Ji S, Kan Y, Chuanling Q, Zhou J-J, Pelosi P (2008) Multiple functions of an odorant-binding protein in the mosquito Aedes aegypti Biochem. Biophys Res Commun 372:464–468. CrossRefGoogle Scholar
  25. Lohr F, Ruterjans H (1995) A new triple-resonance experiment for the sequential assignment of backbone resonances in proteins. J Biomol NMR 6:189–197. CrossRefGoogle Scholar
  26. Marsh JA, Singh VK, Jia Z, Forman-Kay JD (2006) Sensitivity of secondary structure propensities to sequence differences between alpha- and gamma-synuclein: implications for fibrillation. Protein Sci 15:2795–2804. CrossRefGoogle Scholar
  27. Muhandiram DR, Kay LE (1994) Gradient-enhanced triple-resonance 3-dimensional nmr experiments with improved sensitivity. J Magn Reson Ser B 103:203–216. CrossRefGoogle Scholar
  28. Murphy EJ, Booth JC, Davrazou F, Port AM, Jones DN (2013) Interactions of Anopheles gambiae odorant-binding proteins with a human-derived repellent: implications for the mode of action of n,n-diethyl-3-methylbenzamide (DEET). J Biol Chem 288:4475–4485. CrossRefGoogle Scholar
  29. Pelosi P, Zhou JJ, Ban LP, Calvello M (2006) Soluble proteins in insect chemical communication. Cell Mol Life Sci 63:1658–1676. CrossRefGoogle Scholar
  30. Petersen TN, Brunak S, von Heijne G, Nielsen H (2011) SignalP 4.0: discriminating signal peptides from transmembrane regions. Nat Methods 8:785–786. CrossRefGoogle Scholar
  31. Plettner E, Lazar J, Prestwich EG, Prestwich GD (2000) Discrimination of pheromone enantiomers by two pheromone binding proteins from the gypsy moth Lymantria dispar. Biochemistry 39:8953–8962CrossRefGoogle Scholar
  32. Pompeia C, Lima T, Curi R (2003) Arachidonic acid cytotoxicity: can arachidonic acid be a physiological mediator of cell death? Cell Biochem Funct 21:97–104. CrossRefGoogle Scholar
  33. Pophof B (2002) Moth pheromone binding proteins contribute to the excitation of olfactory receptor cells. Naturwissenschaften 89:515–518ADSCrossRefGoogle Scholar
  34. Pophof B (2004) Pheromone-binding proteins contribute to the activation of olfactory receptor neurons in the silk moths Antheraea polyphemus and Bombyx mor. Chem Senses 29:117–125 iCrossRefGoogle Scholar
  35. Sandler BH, Nikonova L, Leal WS, Clardy J (2000) Sexual attraction in the silkworm moth: structure of the pheromone-binding-protein-bombykol complex. Chem Biol 7:143–151CrossRefGoogle Scholar
  36. Serth J, Lautwein A, Frech M, Wittinghofer A, Pingoud A (1991) The inhibition of the GTPase activating protein-Ha-ras interaction by acidic lipids is due to physical association of the C-terminal domain of the GTPase activating protein with micellar structures. EMBO J 10:1325–1330CrossRefGoogle Scholar
  37. Shanbhag SR et al (2001) Expression mosaic of odorant-binding proteins in Drosophila olfactory organs. Microsc Res Tech 55:297–306CrossRefGoogle Scholar
  38. Sim S, Ramirez JL, Dimopoulos G (2012) Dengue virus infection of the Aedes aegypti salivary gland and chemosensory apparatus induces genes that modulate infection and blood-feeding. Behavior PLoS Path 8:e1002631. CrossRefGoogle Scholar
  39. Smallegange RC, van Gemert GJ, van de Vegte-Bolmer M, Gezan S, Takken W, Sauerwein RW, Logan JG (2013) Malaria infected mosquitoes express enhanced attraction to human odor. PLoS ONE 8:e63602. ADSCrossRefGoogle Scholar
  40. Studier FW, Rosenburg AH, Dunn JJ, Dubendorff JW (1990) Use of T7 RNA polymerase to direct expression of cloned genes. Methods Enzymol 185:61–89Google Scholar
  41. Swarup S, Williams TI, Anholt RRH. Genes (2011) Functional dissection of Odorant binding protein genes in Drosophila melanogaster. Brain Behavior 10:648–657. Google Scholar
  42. Verhulst NO et al (2013) Relation between HLA genes, human skin volatiles and attractiveness of humans to malaria mosquitoes. Infect Genet Evol 18:87–93. CrossRefGoogle Scholar
  43. Vögeli B, Güntert P, Riek R (2013) Multiple-state ensemble structure determination from eNOE spectroscopy. Mol Phys 111:437–454. ADSCrossRefGoogle Scholar
  44. Vogt RG, Riddiford LM (1981) Pheromone binding and inactivation by moth antennae. Nature 293:161–163ADSCrossRefGoogle Scholar
  45. Vranken WF et al (2005) The CCPN data model for NMR spectroscopy: development of a software pipeline. Proteins 59:687–696CrossRefGoogle Scholar
  46. Wojtasek H, Leal W (1999) Conformational change in the pheromone-binding protein from Bombyx mori induced by pH and by interaction with membranes. J Biol Chem 274:30950–30956CrossRefGoogle Scholar
  47. Xu P, Atkinson R, Jones DNM, Smith DP (2005) Drosophila OBP LUSH is required for activity of pheromone-sensitive. Neurons Neuron 45:193–200. CrossRefGoogle Scholar
  48. Yamazaki T, Forman-Kay JD, Kay LE (1993) Two-dimensional NMR experiments for correlating carbon-13.beta. and chemical shifts of aromatic residues in 13C-labeled proteins via scalar couplings. J Am Chem Soc 115:11054–11055. CrossRefGoogle Scholar
  49. Yang G, Winberg G, Ren H, Zhang S (2011) Expression, purification and functional analysis of an odorant binding protein AaegOBP22 from Aedes aegypti. Protein Expr Purif 75:165–171. CrossRefGoogle Scholar
  50. Ziegelberger G (1995) Redox-shift of the pheromone-binding protein in the Silkmoth Antheraea-Polyphemus. Eur J Biochem 232:706–711CrossRefGoogle Scholar
  51. Zwahlen C, Legault P, Vincent SJF, Greenblatt J, Konrat R, Kay LE (1997) Methods for measurement of intermolecular NOEs by multinuclear NMR spectroscopy: Application to a bacteriophage lambda N-peptide/boxB RNA complex J Am Chem Soc 119:6711–6721CrossRefGoogle Scholar

Copyright information

© The Author(s) 2019

OpenAccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (, 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.Department of PharmacologyUniversity of Colorado School of MedicineAuroraUSA
  2. 2.Program in Structural Biology and BiochemistryUniversity of Colorado School of MedicineAuroraUSA

Personalised recommendations