Abstract
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.
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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).
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.
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.
Discussion
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.
Change history
02 April 2019
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02 April 2019
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References
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. https://doi.org/10.1016/0022-2364(87)90225-3
Berg MJVD, Ziegelberger G (1991) On the function of the pheromone binding protein in the olfactory hairs of Antheraea polyphemus. J Insect Physiol 37:79–85
Braks MA, Anderson RA, Knols BG (1999) Infochemicals in mosquito host selection: human skin microflora and Plasmodium parasites. Parasitol Today 15:409–413
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 276:20078–20084
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. https://doi.org/10.1021/bi201115q
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. https://doi.org/10.1110/ps.9.5.1038
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 6:277–293
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. https://doi.org/10.1021/ja00042a003
Grzesiek S, Bax A (1992b) Improved 3D triple-resonance NMR techniques applied to a 31-KDa protein. J Magn Reson 96:432–440. https://doi.org/10.1016/0022-2364(92)90099-S
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. https://doi.org/10.1007/BF00178261
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. https://doi.org/10.1006/jmrb.1993.1019
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 12:1357–1369
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 28:479–489
Horst R et al (2001) NMR structure reveals intramolecular regulation mechanism for pheromone binding and release. Proc Natl Acad Sci USA 98:14374–14379
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. https://doi.org/10.1021/ja908004w
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. https://doi.org/10.1007/s10858-012-9611-z
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. https://doi.org/10.1016/j.jmr.2013.11.014
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. https://doi.org/10.1021/ja00033a019
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. https://doi.org/10.1021/ja00052a088
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. https://doi.org/10.1038/nsb960
Lacroix R, Mukabana WR, Gouagna LC, Koella JC (2005) Malaria infection increases attractiveness of humans to mosquitoes. PLoS Biol 3:e298. https://doi.org/10.1371/journal.pbio.0030298
Larter NK, Sun JS, Carlson JR (2016) Organization and function of Drosophila odorant binding proteins. eLife 5. https://doi.org/10.7554/eLife.20242
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. https://doi.org/10.1016/j.cell.2008.04.046
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. https://doi.org/10.1016/j.bbrc.2008.05.064
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. https://doi.org/10.1007/BF00211783
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. https://doi.org/10.1110/ps.062465306
Muhandiram DR, Kay LE (1994) Gradient-enhanced triple-resonance 3-dimensional nmr experiments with improved sensitivity. J Magn Reson Ser B 103:203–216. https://doi.org/10.1006/jmrb.1994.1032
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. https://doi.org/10.1074/jbc.M112.436386
Pelosi P, Zhou JJ, Ban LP, Calvello M (2006) Soluble proteins in insect chemical communication. Cell Mol Life Sci 63:1658–1676. https://doi.org/10.1007/s00018-005-5607-0
Petersen TN, Brunak S, von Heijne G, Nielsen H (2011) SignalP 4.0: discriminating signal peptides from transmembrane regions. Nat Methods 8:785–786. https://doi.org/10.1038/nmeth.1701
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 39:8953–8962
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. https://doi.org/10.1002/cbf.1012
Pophof B (2002) Moth pheromone binding proteins contribute to the excitation of olfactory receptor cells. Naturwissenschaften 89:515–518
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 i
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 7:143–151
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 10:1325–1330
Shanbhag SR et al (2001) Expression mosaic of odorant-binding proteins in Drosophila olfactory organs. Microsc Res Tech 55:297–306
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. https://doi.org/10.1371/journal.ppat.1002631.t001
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. https://doi.org/10.1371/journal.pone.0063602
Studier FW, Rosenburg AH, Dunn JJ, Dubendorff JW (1990) Use of T7 RNA polymerase to direct expression of cloned genes. Methods Enzymol 185:61–89
Swarup S, Williams TI, Anholt RRH. Genes (2011) Functional dissection of Odorant binding protein genes in Drosophila melanogaster. Brain Behavior 10:648–657. https://doi.org/10.1111/j.1601-183X.2011.00704.x
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. https://doi.org/10.1016/j.meegid.2013.05.009
Vögeli B, Güntert P, Riek R (2013) Multiple-state ensemble structure determination from eNOE spectroscopy. Mol Phys 111:437–454. https://doi.org/10.1080/00268976.2012.728257
Vogt RG, Riddiford LM (1981) Pheromone binding and inactivation by moth antennae. Nature 293:161–163
Vranken WF et al (2005) The CCPN data model for NMR spectroscopy: development of a software pipeline. Proteins 59:687–696
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 274:30950–30956
Xu P, Atkinson R, Jones DNM, Smith DP (2005) Drosophila OBP LUSH is required for activity of pheromone-sensitive. Neurons Neuron 45:193–200. https://doi.org/10.1016/j.neuron.2004.12.031
Yamazaki T, Forman-Kay JD, Kay LE (1993) Two-dimensional NMR experiments for correlating carbon-13.beta. and proton.delta./.epsilon. chemical shifts of aromatic residues in 13C-labeled proteins via scalar couplings. J Am Chem Soc 115:11054–11055. https://doi.org/10.1021/ja00076a099
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. https://doi.org/10.1016/j.pep.2010.09.004
Ziegelberger G (1995) Redox-shift of the pheromone-binding protein in the Silkmoth Antheraea-Polyphemus. Eur J Biochem 232:706–711
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 119:6711–6721
Acknowledgements
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).
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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.
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Jones, D.N.M., Wang, J. & Murphy, E.J. Complete NMR chemical shift assignments of odorant binding protein 22 from the yellow fever mosquito, Aedes aegypti, bound to arachidonic acid. Biomol NMR Assign 13, 187–193 (2019). https://doi.org/10.1007/s12104-019-09875-0
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DOI: https://doi.org/10.1007/s12104-019-09875-0