http://orcid.org/0000-0001-8599-2771
Figures
Abstract
NADPH–cytochrome P450 reductase (CPR) plays an important role in the cytochrome P450 (CYP)-mediated metabolism of endogenous and exogenous substrates. CPR has been found to be associated with insecticide metabolism and resistance in many insects. However, information regarding CPR in the bird cherry-oat aphid, Rhopalosiphum padi, is unavailable. In the current study, a full-length cDNA (2,476 bp) of CPR (RpCPR) encoding 681 amino acids was cloned from R. padi. Nucleotide sequence and deduced amino acid sequence analysis showed that RpCPR exhibits characteristics of classical CPRs and shares high identities with those of other insects, especially with the pea aphid, Acyrthosiphon pisum. The mRNA of RpCPR was expressed at all developmental stages, with the highest expression level found in the second instar and the lowest in adult. Expression levels of RpCPR in isoprocarb-resistant and imidacloprid-resistant strains were 3.74- and 3.53-fold higher, respectively, than that of a susceptible strain. RpCPR expression could also be induced by low concentrations (LC30) of isoprocarb and imidacloprid. Moreover, we sequenced the open reading frame (ORF) of RpCPR from 167 field samples collected in 11 geographical populations. Three hundred and thirty-four SNPs were detected, of which, 65 were found in more than two individuals. One hundred and ninety-four missense mutations were present in the amino acid sequence, of which, the P484S mutant had an allele frequency of 35.1%. The present results suggest that RpCPR may play an important role in the P450-mediated insecticide resistance of R. padi to isoprocarb and imidacloprid and possibly other insecticides. Meanwhile, RpCPRmaintains high genetic diversity in natural individuals, which provides the possibility of studying potential correlations between variants and certain special physiological characters.
Citation: Wang K, Peng X, Zuo Y, Li Y, Chen M (2016) Molecular Cloning, Expression Pattern and Polymorphisms of NADPH-Cytochrome P450 Reductase in the Bird Cherry-Oat Aphid Rhopalosiphum padi (L.). PLoS ONE 11(4): e0154633. https://doi.org/10.1371/journal.pone.0154633
Editor: Claude Wicker-Thomas, CNRS, FRANCE
Received: December 29, 2015; Accepted: April 15, 2016; Published: April 28, 2016
Copyright: © 2016 Wang et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: All relevant data are within the paper and its Supporting Information files.
Funding: This work was funded by the National Natural Science Foundation of China (grant nos. 31471766 and 31272036), the Doctoral Program Foundation of Institutions of Higher Education of China (grant no. 20110204110001) and the National Key Technology R&D Program of the Ministry of Science and Technology (grant no. 2012BAK11B03). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Introduction
The bird cherry-oat aphid, Rhopalosiphum padi (L.), is one of the most important pests of wheat in temperate regions worldwide [1]. Aside from direct feeding damage, R. padi also transmits the barley yellow dwarf virus (BYDV), which causes economically important disease of small grains and leads to significantly reduced quality and yield [2–4]. To minimize economic losses, multiple types of insecticides are chronically and excessively used in aphid control in modern agriculture. Insecticide resistance or changes in insecticide susceptibility have been documented occasionally in R. padi and other wheat aphids in various parts of the world, and is a long-standing challenge for chemical pest management in aphids and other agricultural pests [5–9].
Many studies suggest that the cytochrome P450 monooxygenase (P450) system is involved in the detoxification of xenobiotics, as well as the metabolism of endogenous compounds. P450-mediated insecticide resistance has been characterized in many insects [10], including aphids [11]. P450s can degrade all classes of insecticides [10,12], and in this metabolic reaction, the iron atom in the heme group of P450 must accept two electrons from NADH/NADPH [13], and NADPH-cytochrome P450 reductase (CPR, also referred to as POR, CYPOR, OR, NCPR, and P450R) functions as an electron transporter (redox partner), accepting electrons from NADPH and transferring them to P450s [14–15]. In some P450s (CYP1A2, CYP3A4, etc.), cytochrome b5 may also act as a donator of a second electron [15,16]. In addition, numerous studies have shown that, although there is an extensive diversity of P450 isoforms, generally only one CPR gene exists in the genome of each creature, including insecta [15,17,18]. Therefore, the CPR gene is considered a vital part of P450-mediated insecticide resistance and is considered a novel target for the development of “smart” insecticides and synergists [19–20]. Inhibition of CPR reduces the activities of all microsomal P450 enzymes. Conditional deletion of CPR in the liver results in the inactivation of the hepatic P450 system [21]. In the bed bug Cimex lectularius and mosquito Anopheles gambiae, silencing of CPR resulted in increased susceptibility to pyrethroid insecticides in resistant populations [18,22]. RNA interference (RNAi) of Nilaparvata lugens CPR significantly reduced the transcription level and resulted in increased sensitivity to beta-cypermethrin and imidacloprid [23]. Additionally, directed RNAi of CPR of some insects significantly affected the biosynthesis of endogenous substances such as pheromone and cuticular hydrocarbon [24,25].
Another fascinating aspect of CPR is its numerous polymorphisms or/and mutations. Since the first report of CPR deficiency [26], many studies worldwide have described the varying phenotypes in humans; to date, over 2,000 single nucleotide polymorphisms (SNPs) have been described in human CPR genes, encompassing over 150 missense mutations that affect transcription, have also been identified in many syndromes [13,15]. However, few polymorphisms or/and mutations in insect CPR genes have been reported.
Genetic information regarding CPR has become available in several insect species since the first report of the cDNA and deduced protein sequence of CPR in the house fly, Musca domestica [27]. The CPR gene of the fruit fly, Drosophila melanogaster [28], silkworm, Bombyx mori [29] and cabbage armyworm, Mamestra brassicae [30] have been cloned and studied in terms of their involvement in odorant clearance and 20-hydroxyecdysone biosynthesis. Recently, the focus on insect CPR genes has shifted to insecticide resistance. Genetic studies of the mosquitos Anopheles gambiae [31] and A. minimusm [32], and bed bug, C. lectularius [18], among others, have shown that CPR is related to resistance to pyrethroid insecticides in public health pests. Meanwhile, more CPR genes were also characterized in agricultural pests such as the rice brown planthopper, Nilaparvata lugens [23] and diamondback moth, P. xylostella [33], and demonstrated to be associated with insecticide resistance. To our knowledge, there is no report concerning the sequences or functions of CPR, nor its polymorphisms or/and mutations in R. padi.
In the present study, R. padi CPR (RpCPR) was cloned and its expression pattern analyzed at various developmental stages. Its expression profiles in an isoprocarb resistant-strain and imidacloprid-resistant strain, in addition to the transcriptional response of RpCPR to the two insecticides in a susceptible strain (SS), were examined. Moreover, the gene polymorphisms or/and mutations in 167 natural individuals of 11 geographical populations in China were evaluated. These data may facilitate further study of the functions of CPR in P450-mediated isoprocarb resistance, imidacloprid resistance and other physiological mechanisms in R. padi. Moreover, the high genetic diversity of RpCPR in natural individuals provides the possibility of testing potential correlations between variants and several unique physiological characteristics.
Materials and Methods
Ethics Statement
No specific permissions were required for the described field studies for this wide spread agriculture pest. We confirm that the locations were not privately owned or protected in any way. The field studies did not involve endangered or protected species.
Aphids
In this study, all Rhopalosiphum padi were reared at 23 ± 1°C, a photoperiod of L16:D8, and relative humidity of 60 ± 5%. Three bird cherry-oat aphid strains were used in this study. An insecticide-susceptible strain (SS) (LC50 values of 0.980 mg/L for imidacloprid and 1.032 mg/L for isoprocarb) first collected in Gansu Province, China in 2013 was maintained in the laboratory for more than three years without insecticide exposure. A imidacloprid-resistant strain (IM-R) and a isoprocarb-resistant strain (IS-R) was generated after continuous treatment with exposure to the respective two insecticides, which regularly kill 40% -70% of aphids, every 15 days. The IM-R strain showed an LC50 value of 21.3 mg /L for imidacloprid, with a resistance ratio of 21.7-fold, and the IS-R strain displayed a 32.4-fold increase in resistance compared to the SS strain, with an LC50 value of 33.4 mg/L for isoprocarb.
To detect RpCPR polymorphisms and mutations, we collected R. padi from 11 geographical populations in various wheat production areas of China (Table 1). All samples were collected from wheat. Each population was collected from at least eight collection points in a wheat field, and five individuals were obtained in each collection point. The distance between any two points was at least 30 m.
RNA Isolation and cDNA Synthesis
Total RNA was extracted using TRIzol reagent (Invitrogen, Carlsbad, CA, USA) according to the manufacturer’s instructions, and was treated with DNase I (Takara, Kyoto, Japan). For real-time quantitative polymerase chain reaction (RT-qPCR) analysis, 2 μg of total RNA (500 μg/mL) were reverse-transcribed into single-stranded cDNA with the reaction mixture containing 2 μL Oligo (dT) (500 μg/mL) and 4 μL distilled water using an M-MLV Reverse Transcriptase cDNA Synthesis Kit (Promega, Madison, WI, USA) according to the manufacturer’s recommendations. For amplification of RpCPR, cDNA was synthesized using a SMARTer™ RACE cDNA Amplification Kit (Clontech, Mountain View, CA, USA). The cDNA synthesized was stored at -20°C.
Cloning of RpCPR
The full-length cDNA of RpCPR was cloned by RT-PCR and rapid amplification of cDNA ends (RACE). Firstly, Specific primers (CPR-F and CPR-R) were designed from the nucleotide sequence of the Acyrthosiphon pisum CPR gene (accession no. XM_001945277.3). Based on the partial putative fragment of RpCPR obtained via primer pair CPR-F and CPR-R, gene-specific primes for 5′-RACE (RpCPR -5R) and 3′-RACE (RpCPR -3R1 and RpCPR -3R2) were designed to clone the of 5′and 3′ sequences of the gene. To confirm the full length of the RpCPR linked from the 5′-RACE and 3′-RACE results, a specific primer pair (RpCPR-CF and RpCPR-CR) was designed to amplify the full length of the gene. All the primers used is showed in Table 2. All PCR products were purified with a Wizard PCR Preps kit (Promega, Madison, WI, USA). The PCR products purified were cloned into pGEM-T easy vectors (Promega, Madison, WI, USA) and transformed into Escherichia coli DH5α competent cells. Five positive clones of each sample were randomly chosen for bidirectional sequencing on an Applied Biosystems 3730 automated sequencer (Applied Biosystems, Foster City, CA, USA).
Sequence Analysis of RpCPR
The full-length cDNA of RpCPR was assembled using DNAMAN version 5.2 (Lynnon Biosoft, San Ramon, CA, USA), and its ORF and deduced amino acid sequence were determined using ORF Finder (http://www.ncbi.nlm.nih.gov/gorf/gorf.html). The theoretical isoelectric point (pI) and molecular weight (MW) of RpCPR were calculated using ExPASy (www.expasy.org/tools/protparam.html). Putative transmembrane domains and signal peptides were predicted with TMHMM (www.cbs.dtu.dk/services/TMHMM-2.0/) and signalP (www.cbs.dtu.dk/services/SignalP/), respectively. The binding domains and catalytic residues were predicted by Conserved Domain Search (www.ncbi.nlm.nih.gov/Structure/cdd/cdd.shtml/). Sequence identification and similarities were analyzed using BLAST (blast.ncbi.nlm.nih.gov/blas). Amino acid sequences of RpCPR and orthologs from other insect species were aligned using ClustalW2 (http://www.ebi.ac.uk/Tools/msa/clustalw2/), and a phylogenetic tree was constructed by the neighbor-joining method with bootstrap test of 1,000 replicates using MEGA 5.0 software [34].
Qualitative Real-Time PCR (qPCR) Analysis
Primers for RT-qPCR were designed using Primer 5 and are listed in Table 2. β-actin was used as the house-keeping gene in the analysis [35].The specificity of primer pairs (RpCPR-qF and RpCPR-qR, actin-F and actin-R) was tested and confirmed by sequencing basing on preliminary experiment (data not shown). RT-qPCR was performed on a LightCycler Nano System (Roche, Mannheim, Germany) with FastStart Essential DNA Green Master (Roche, Mannheim, Germany) in accordance with the manufacturer’s instructions. Using 20-fold-diluted cDNA as templates, all reactions were performed in a 20 μL final volume including 10 μL FastStart Essential DNA Green Master, 0.8 μL each specific primer (Table 2), 2 μL cDNA template, and 6.4 μL RNase-free water. The reaction was performed at 95°C for 3 min, followed by 40 cycles of 10 s at 95°C, 20 s at 58°C and 20 s at 72°C; a final melt-curve step was included post-PCR (ramping from 55°C to 95°C by 0.5°C every 5 s) to check for nonspecific amplification. Each reaction was performed in triplicate, after which the average threshold cycle (Ct) per sample was calculated. The β-actin gene of R. padi was used as the internal control gene to normalize the target gene expression levels. The relative expression of genes was calculated using 2−ΔΔCt method. Three biological replicates were run for each experiment.
RpCPR Expression in Different Development Stages and Different Strains
To investigate the expression pattern of RpCPR at various developmental stages, the relative transcript levels if the gene in all the five developmental stages (1st, 2nd, 3rd and 4th instar, and adult) of the R. padi were investigated by RT-qPCR. Total RNA was isolated from individuals (5 mg) of each developmental stages of SS strain. The aforementioned methods for RNA extraction and qPCR were used.
The relative expression level of RpCPR in IS-R, IM-R and SS strains was analyzed using qRT-PCR. Total RNA was isolated from individuals (5 mg) of each strain. The methods for RNA extraction and qPCR were as described above.
RpCPR Expression after Exposure to Isoprocarb and imidacloprid
Isoprocarb and imidacloprid used in the study were of technical grade. The neonicotinoid, imidacloprid (95% purity), was provided by Jiangsu Changlong Chemical Co., Ltd., China. The carbamate, isoprocarb (95% purity), was provided by Anhui Huaxing Chemical Industry Co., Ltd., China.
Standard stock solutions (10 g/L) of each insecticide were prepared in acetone. Then, stock solutions were further diluted to the LC30 (0.567 mg/L for isoprocarb and 0.363 mg /L for imidacloprid) concentration using 0.1% Triton X-100 solution, with 0.0057% (v/v) acetone in isoprocarb solution and 0.0036% (v/v) acetone in imidacloprid solution, respectively. All solutions were stored in the dark at 4°C.
The previously reported leaf-dipping method was adopted for treatment [35,36]. Wheat leaves with apterous adult aphids (SS) were dipped into the aforementioned LC30 solutions which can killed around 30% of the aphids for 10 s, after which the leaves were taken out and residual solution droplets on the leaf were adsorbed using clean, dry filter paper. Leaves were dipped into 0.1% Triton X-100 only for use as controls. Three replicates of 50–60 aphids each were used for each chemical and control treatment. All aphids were maintained at a constant temperature of 23 ± 1°C and a photoperiod of 16:8 (L: D) h during and after treatment. Live aphids were collected at 3, 6, 12, and 24 h post-treatment, total RNA was isolated from individuals (5 mg) of the live aphids collected at each treatment, and the CPR expression level was analyzed. The methods for RNA extraction and qPCR were as described above.
Polymorphism or/and Mutation Identification
RNA was isolated from apterous adult aphid from different geographical populations in China, and reverse-transcripted as described above. PCR amplification was performed using Takara LA-Taq DNA Polymerase (Takara Bio, Dalian, China) under cycling conditions of 5 min at 94°C followed by 30 cycles of 30 s at 94°C, 30 s at 55°C and 1 min at 72°C. PCR products were purified using a Wizard PCR Preps Kit (Promega, Madison, WI, USA), and the purified fragments were cloned into a pGEM-Teasy Vector (Promega, Madison, WI, USA) and transformed into Escherichia coli JM109. Finally, two recombinant plasmids with each insert were sequenced by Sangon Biotech (Shanghai, China) [37].
The nucleotide and acid amino sequences of the SS strain were used as the standard models. All nucleotide sequences were aligned with ClustalX, and SNPs and haplotypes were ascertained using DnaSP v5 [38] and MEGA 5.0 software.
Statistical Analyses
Data analyses were carried out using SPSS statistics software (SPSS Inc., Chicago, IL, USA). For RT-qPCR results, all data were subjected to one-way analysis of variance (ANOVA) with the least significant difference test among multiple groups or analyzed by Student’s t-test (two-tailed paired t-test) between two groups and are expressed as the mean ± standard error (SE). The level of significance was set at P<0.05.
Results
Cloning and Sequence Analysis of R. padi CPR
A partial putative cDNA fragment of R. padi CPR (~650 bp) was amplified from apterous adult aphids (SS strain) by PCR using specific primers (CPR-F and CPR-R) designed based on the homologous gene sequence in A. pisum. BLAST analysis of the nucleotide sequence of the partial putative RpCPR cDNA showed that the sequence shared 94% nucleotide similarity with the corresponding sequence from the pea aphid. The complete cDNA of RpCPR has a 5′-untranslated region (5′-UTR) of 330 bp, a 3′-untranslated region (3′-UTR) of 103 bp, and an ORF of 2,046 bp, which encodes a protein of 681 amino acids. The pI and MW of RpCPR were predicted to be 5.27 and 77.11 kDa, respectively. The nucleotide sequence of R. padi CPR has been deposited into GenBank under accession number KU057505.
The RpCPR protein possesses several characteristic structural features. Multiple alignment of RpCPR and several other known CPRs (CRR of M. domestica, D. melanogaster and Rattus norvegicus) (Fig 1B) showed that RpCPR shares high identity with two other insect CPRs, and the three binding domains are conserved in the CPRs of insects and rats. No signal peptide was found within RpCPR, but the membrane anchor that facilitates the localization of RpCPR on the endoplasmic reticulum (ER) was identified at the N-terminus (Fig 1A). The amino acid residues arginine 457, tyrosine 459 and serine 460 constituted the consensus binding site of the flavin adenine dinucleotide (FAD)-binding motif, which is ubiquitous in the FAD-binding domain [39] (Fig 1A). Four catalytic residues (serine 460, cysteine 631, aspartic 676, and tryptophan 678) (Fig 1A) formed the active site, which has been demonstrated to be critical in the hydride transfer reaction [40,41].
(A) Schematic drawing of RpCPR. Membrane anchor, conserved FMN-, FAD- and NADP-binding domains, FAD-binding motif (Arg457 x Tyr459 Ser456), and catalytic residues (Ser460, Cys633, Asp678 and Trp680) are shown. (B) Comparison of the deduced amino acid sequence of RpCPR with those of other CPRs deposited into GenBank. The species and accession numbers are as follows: Musca domestica (NP_001273818), Drosophila melanogaster (NP_477158) and Rattus norvegicus (NP_113764).
Phylogenetic Relationship between RpCPR and Other Insect CPRs
Phylogenetic analysis was performed using MEGA 5.0 software based on the deduced amino acid sequences of RpCPR and 38 other insect CPRs (S1 Table). The neighbor-joining phylogenetic tree showed that CPRs from the same insect order were clustered in the same branch (Fig 2). RpCPR and pea aphid A. pisum CPR were grouped together with strong bootstrap support (100%).
The neighbor-joining tree was generated using MEGA 5.0 software, and the phylogeny was tested by the bootstrap method with 1,000 replications. Bootstrap values >50% are shown. R. padi CPR is indicated by solid circles. The GenBank accession numbers of the sequences used were listed in supporting information S1 Table.
Developmental Expression Profiles of R. padi CPR
Insect P450s mediate a series of metabolic processes during the whole insect life cycle, and as an important electron transfer partner, the development-related expression profile of CPR could be a reflection of P450 activity [23]. RpCPR transcripts were detected at all developmental stages including the 1st, 2nd, 3rd, 4th instar and adult (Fig 3), and the transcript level rapidly increased from the first to second instar, and then gradually decreased from the second instar to adult. The expression level of RpCPR in the second instar was 5.01-fold higher than in other stages (P< 0.05).
Relative expression levels of RpCPR at different developmental stages were normalized to those in the adult. Data shown as the mean ± SE; different letters denoted a significant difference among samples (P<0.05, one-way ANOVA).
Expression of RpCPR in the IS-R, IM-R and SS Strains
The expression levels of RpCPR in the apterous adult aphids of the IS-R, IM-R and SS strains were analyzed. RpCPR expression was significantly higher in IS-R and IM-R than in SS (P<0.05), with increases of 3.74- and 3.52-fold, respectively, indicating its potential involvement in isoprocarb and imidacloprid resistance (Fig 4).
The expression level of RpCPR in SS was set to 1. Data shown as the mean ± SE; different letters denoted a significant difference among samples (P<0.05, one-way ANOVA).
Effect of Isoprocarb and Imidacloprid on RpCPR Expression
Apterous adult aphids of the SS strain were exposed to the LC30 concentrations of isoprocarb and imidacloprid. RpCPR expression increased 1.66- to 2.18-fold after exposure to the isoprocarb (Fig 5). The RpCPR mRNA level was significantly increased at 3 h (1.85-fold) and 6 h (2.08-fold) after imidacloprid treatment, and then recovered to a normal level at 12 h (1.16-fold) and 24 h (1.19-fold) (Fig 5).
Data shown as the mean ± SE; different letters denoted a significant difference among samples (P<0.05, one-way ANOVA). The expression level of RpCPR in SS strain marked with a dash line at Y = 1.0.
RpCPR Polymorphisms in Field Samples
We sequenced the coding region of RpCPR from 167 individuals of 11 geographic populations in China (Table 1; GenBank accession numbers KU057506–KU057672). There were 146 haplotypes in the 167 individuals, and 334 distinct nucleotide variable sites were identified in the sequence (Table 1). Of these variable (polymorphic) sites, only 65 were detected in more than two individuals in the total population, and most were detected in one individual. The most common variants, A627T, G1362A, C1450T, and A1536T, were found in 31.7%, 35.3%, 35.3%, and 30.5% of the haplotypes, respectively.
Missense mutations or/and polymorphisms in the amino acid sequence of RpCPR using the amino sequence of the SS strain as the standard are shown in Fig 6. In total, 194 missense mutations were found in the 167 aphid individuals, of which, 31 missense mutations belonged to parsimony-informative sites. Specifically, the amino acid sequence variant Pro484Ser, which resulted from the nucleotide variant C1450T, was found in 59 individuals from 11 geographic populations.
Mutation found only in one individual is indicated by a hollow triangle while polymorphic variants identified in more than two individuals are indicated by a solid triangle. The digital number after the mutated amino acids indicated the number of the aphid individuals with the mutation.
Discussion
The cytochrome P450-mediated metabolic system is a major mechanism of insecticide resistance and the only system that can mediate resistance to all classes of insecticides [10]. In aphids, 83, 115 and 66 P450 genes were identified in pea aphid (A. pisum), green peach aphid (Myzus persicae) and cotton aphid (Aphis gossypii), respectively [42,43]. The CYP6CY3 gene is associated with resistance to neonicotinoid insecticides in M. persicae [11, 44]. In the mono-oxygenation reaction, CPR is indispensable, as it functions as a unique electron transporter for almost all microsomal P450s [15]. Analysis of the function of insect CPR would enable further evaluation of the mechanism of insecticide resistance and facilitate the identification of new targets for insecticides.
In this study, the RpCPR gene was isolated from R. padi. Alignment analysis showed high identities of the deduced amino acid sequence of RpCPR with those of other insect CPRs. The phylogenetic analysis demonstrated that RpCPR and other hemipteran CPRs were clustered together within the branch for Hemiptera. Structure prediction indicated that RpCPR contains a membrane anchor in the N-terminal transmembrane region comprising 20 amino acid residues. Due to this hydrophobic segment, the remainder of CPR likely faces the cytoplasmic side of the membrane of the ER [45,46], which is important for electron transfer. Microsomal P450s are also inserted into the ER membrane by the N-terminal anchor sequence [13,47]. FMN (flavin mononucleotide)-binding, FAD-binding and NADPH (nicotinamide adenine dinucleotide phosphate)-binding domains were identified in the hydrophilic C-terminal catalytic domain of RpCPR, and alignment analysis with three classical CPRs demonstrated that these binding domains are highly conserved among the CPRs of insects and mammals (Fig 1). The FMN-binding domain of RpCPR comprises two conserved binding sites including the FMN ring (si-face) and FMN ring (re-face), which are critical for the interaction with the redox-partner binding site of P450s [48]. Electrons derived from NADPH in the form of two hydride ions are transferred to FAD, then to FMN. The electrons are then delivered one at a time to P450s or other acceptors [49–51]. The deduced amino acid sequence of R. padi CPR showed the highest identity to the CPR of A. pisum, which is consistent with the phylogenetic analysis results, showing that they cluster to the same monophyletic group (Fig 1). It is likely that these proteins perform similar physiological functions.
For the first time, we examined the expression profile of CPR mRNA in different developmental stages in an aphid species. RpCPR was expressed at various levels in R. padi during five life stages, likely due to different metabolic requirements at different developmental stages. RpCPR are involved in various demands of different P450s, which catalyze various endogenous biosynthesis and metabolic reactions. Insect Halloween P450 enzymes mediated the sequential hydroxylations of steroid precursors into the active ecdysteroid, 20-hydroxyecdysone [52,53]. CYP15A1, a P450 gene catalyzed epoxidation of methyl farnesoate to juvenile hormone in Diploptera punctata [54]. These two hormones governed the larval molting and metamorphosis. CPR genes of different insect species have diverse expression profiles throughout the life cycle. The expression levels of N. lugens CPR fluctuated during developmental stages; NlCPR transcription was highest in the first nymph and lowest in macropterous adults [23]. In C. lectularius, the CPR gene was ubiquitously expressed in all life stages, and its expression increased as immature stages developed into adults [18].
For detoxifying exogenous compounds such as insecticides in insects, the constitutively increased expression of P450 genes is thought to be directly linked to the degree of adaptation to the stress in question [55–58]. RpCPR was not only constitutively overexpressed in the imidacloprid- and isoprocarb-resistant strains but also significantly induced by both insecticides. Chen and Zhang (2015) found that P. xylostella CPR could be efficiently induced by a low dose of beta-cypermethrin, and was highly overexpressed in a field-collected beta-cypermethrin-resistant population, it was possible that the over-expression of CPR in resistant insects could effectively enhance P450 metabolism of insecticides [33]. Aside from CPRs, several insect P450 genes are overexpressed in insecticide-resistant strains and can be induced by chemical insecticides. The constitutive expression of CYP6A1 in the house fly M. domestica is at least 10-fold higher in the resistant strain than the susceptible strain, and the gene is inducible by phenobarbital treatment of the flies [59]. Multiple P450 genes including CYP6AA7, CYP9J40, CYP9J34, and CYP9M10 showed constitutive overexpression and permethrin induction in the insecticide-resistant mosquito, Culex quinquefasciatus [57]. Therefore, RpCPR is likely involved in imidacloprid and isoprocarb resistance in R. padi. Further investigations that include the use of RNAi [18,28], transcriptomics [60,61] and metabolomics [62] are required to identify the underlying mechanism. CPR is indispensible for the function of P450s, and CPR inhibitors may enable P450-meditated insecticide resistance to be overcome in insect species.
Our analysis of RpCPR in 167 individuals from 11 geographic populations identified 334 SNPs, 194 of which belonged to nonsynonymous sites, which altered the encoded amino acid sequence. Most of these SNPs were found in only a single sample, while 65 SNPs were found in no fewer than two individuals of the total population. In particular, four SNPs (A627T, G1362A, C1450T, and A1536T) were present in ≥51 individuals, and the C1450T mutation resulted in the amino acid mutation Pro484Ser. More than 35% of individuals from different geographic populations harbored this missense mutation. Pro484Ser is located in the adenine ring (FAD-binding region), which is an important cofactor-binding region in the CPR family [45]. To date, few studies on the functions of CPR missense mutations in invertebrates have been conducted. Several synonymous mutations were detected in a fenvalerate-resistant strain of H. armigera [63]. Some site-directed mutations of A. minimus could enhance FAD or/and FMN binding by CRP, which suggests that CYP6AA3 mediates benzyloxyresorufin O-deakylation [64,65]. However, there are abundant reports of human CPR mutations. A total of over 2,000 SNPs, encompassing over 150 missense mutations, have been described in human CPR [15]. In human CPR, the Y181D mutation, found in patients with congenital adrenal hyperplasia, lacks FMN-binding activity [66]. The A287P, R457H, Y459H, and V492E mutations, which lie in the FAD-binding domain, greatly decrease FAD-binding affinity and disrupt both the 17α-hydroxylase and 17, 20 lyase activities of P450c17 [26,67]. Moreover, the overall 3D structures of some variants are similar to that of the wild type, while some subtle but significant differences exist, including local disruption of hydrogen bonding or/and salt bridging involving the FAD pyrophosphate moiety, leading to weaker FAD binding, an unstable protein and loss of catalytic activity [67,68]. A previous study on the common mutation in human CPR, A503V, which had an allele frequency of ~27% in 842 healthy unrelated humans, showed that the variant modestly but significantly decreased its catalytic activity, which may contribute to individual variations in drug response [69]. Additionally, in the CPR of Saccharomyces cerevisiae, T71A and D187A mutations in the FMN-binding site resulted in almost complete loss of function toward CYP51 [48]. The polymorphism of human CPR could affect activity of some P450s or contributed to some human diseases or human variations to drug response, however, research about the effect of insect CPR gene mutations is rare. In this study, we report insect CPR polymorphisms in field samples, particularly some mutation sites, in several vital regions of RpCPR, indicating the genetic diversity of CPR in insects and a correlation between CPR mutations and insecticide metabolism or/and resistance. Further studies are needed to address the questions raised by our findings. For example, why there are so many mutations in RpCPR? Does insecticide selection pressure cause these mutations? PCR products were purified? Are abundant polymorphisms of CPR common in other insect species?
Conclusions
The present study provides preliminary information on the sequence, phylogenetic relationships and expression pattern of CPR in the bird cherry-oat aphid, R. padi. The gene was overexpressed in the isoprocarb- and imidacloprid-resistant strains. Its expression was induced by sublethal concentrations of isoprocarb or/and imidacloprid. Our results indicate that RpCPR might be involved in resistance to isoprocarb or/and imidacloprid in R. padi. Furthermore, we examined the genetic diversity of RpCPR in several natural populations and described multiple mutation and polymorphism sites. Further studies are needed to investigate RpCPR variants with particular reference to the detoxification or/and activation of xenobiotics, as well as the metabolism of endogenous compounds. Indeed, further studies should assess the function of the RpCPR gene in individual P450-mediated detoxification pathways and other physiological processes in R. padi.
Acknowledgments
We thank Huimin Shen, Jin Huang, Geng Tao, Lijun Chen, Yunzhuan He, Shuxia Tao, Changchun Dai, Fengshan Yang, and JinhuaYang for their help with the collection of Rhopalosiphum padi samples.
Author Contributions
Conceived and designed the experiments: KW XP MC. Performed the experiments: KW. Contributed reagents/materials/analysis tools: KW YL MC. Wrote the paper: KW YZ MC.
References
- 1.
Blackman RL, Eastop VF. Aphids on the world's crops. An identification and information guide. John Wiley; 1984.
- 2. Rochow WF. Biological properties of four isolates of barley yellow dwarf virus. Phytopathology. 1969; 59: 1580–1589. pmid:5377734
- 3. Du ZQ, Li L, Liu L, Wang XF, Zhou G. Evaluation of aphid transmission abilities and vector transmission phenotypes of barley yellow dwarf viruses in China. J Plant Pathol. 2007; 89: 251–259.
- 4. Medina-Ortega KJ, Bosque-Pérez NA, Ngumbi E, Jiménez-Martínez ES, Eigenbrode SD. Rhopalosiphum padi (Hemiptera: Aphididae) responses to volatile cues from barley yellow dwarf virus–infected wheat. Environ Entomol. 2009; 38: 836–845. pmid:19508794
- 5. Brattsten LB, Holyoke CW, Leeper JR, Raffa KF. Insecticide resistance: challenge to pest management and basic research. Science. 1986; 231: 1255–1260. pmid:17839561
- 6. Sekun NP, Kudel KA, Satsyuk OS, Mel'nikova GL, Zil'bermints IV, Zhuravleva LM. A study on potential resistance of cereal aphids to insecticides. Zashchita Rasteniĭ (Kiev). 1990; 37: 49–53.
- 7. Chen MH, Han ZJ, Qiao XF, Qu MJ. Mutations in acetylcholinesterase genes of Rhopalosiphum padi resistant to organophosphate and carbamate insecticides. Genome. 2007; 50: 172–179. pmid:17546082
- 8.
Foster SP, Devine G, Devonshire AL. Insecticide resistance in aphids. In: van Emden HF, Harrington R, editors. Aphids as crop pests. CABI, Wallingford, Oxon, UK; 2007. pp. 261–285.
- 9. Sukhoruchenko GI, Dolzhenko VI. Problems of resistance development in arthropod pests of agricultural crops in Russia. EPPO Bull. 2008; 38: 119–126.
- 10. Li X, Schuler MA, Berenbaum MR. Molecular mechanisms of metabolic resistance to synthetic and natural xenobiotics. Annu Rev Entomol. 2007; 52: 231–253. pmid:16925478
- 11. Puinean AM, Foster SP, Oliphant L, Denholm I, Field LM, Millar NS, et al. Amplification of a cytochrome P450 gene is associated with resistance to neonicotinoid insecticides in the aphid Myzus persicae. Plos Genet. 2010; 6: e1000999. pmid:20585623
- 12.
Feyereisen R. Insect cytochrome P450. In: Gilbert LI, Latrou K, Gill SS, editors. Comprehensive molecular insect science, Vol. 4, ed. Oxford, UK; 2005. pp. 1–77.
- 13. Pandey AV, Flück CE. NADPH P450 oxidoreductase: Structure, function, and pathology of diseases. Pharmacol Therapeut. 2013; 138: 229–254.
- 14. Pompon D, Louerat B, Bronine A, Urban P. Yeast expression of animal and plant P450s in optimized redox environments. Method Enzymol. 1996; 272: 51–64.
- 15.
Waskell L, Kim JJP. Electron transfer partners of cytochrome p450. In: Paul R, Montellano OD, editors. Cytochromes P450: Stucture, Mechanism and Biochemistry. 4rd ed. Springer International Publishing; 2015. pp. 33–68.
- 16. Porter TD. The roles of cytochrome b5 in cytochrome P450 reactions. J Biochem Mol Toxic. 2002; 16: 311–316.
- 17. Backes WL, Kelley RW. Organization of multiple cytochrome P450s with NADPH-cytochrome P450 reductase in membranes. Pharmacol Therapeut. 2003; 98: 221–233.
- 18. Zhu F, Sams S, Moural T, Haynes KF, Potter MF, Palli SR. RNA interference of NADPH-cytochrome P450 reductase results in reduced insecticide resistance in the bed bug, Cimex lectularius. PloS one. 2012; 7: e31037. pmid:22347424
- 19. Lycett GJ, McLaughlin LA, Ranson H, Hemingway J, Kafatos FC, Loukeris TG, et al. Anopheles gambiae P450 reductase is highly expressed in oenocytes and in vivo knockdown increases permethrin susceptibility. Insect Mol Biol. 2006; 15: 321–327. pmid:16756551
- 20. Lian LY, Widdowson P, McLaughlin LA, Paine MJ. Biochemical comparison of Anopheles gambiae and human NADPH P 450 reductases reveals different 2′-5′-ADP and FMN binding traits. Plos one. 2011; 6: e20574. pmid:21655236
- 21. Henderson CJ, Otto DM, Carrie D, Magnuson MA, McLaren AW, Rosewell I, et al. Inactivation of the hepatic cytochrome P450 system by conditional deletion of hepatic cytochrome P450 reductase. J Biol Chem. 2003; 278: 13480–13486. pmid:12566435
- 22. Lycett GJ, McLaughlin LA, Ranson H, Hemingway J, Kafatos FC, Loukeris TG, et al. Anopheles gambiae P450 reductase is highly expressed in oenocytes and in vivo knockdown increases permethrin susceptibility. Insect Mol boil. 2006; 15: 321–327.
- 23. Liu S, Liang Q, Zhou W, Jiang Y, Zhu Q, Yu H, et al. RNA interference of NADPH–cytochrome p450 reductase of the rice brown planthopper, Nilaparvata lugens, increases susceptibility to insecticides. Pest Manag Sci. 2015; 71: 32–39. pmid:24515640
- 24. Sandstrom P, Welch WH, Blomquist GJ, Tittiger C. Functional expression of a bark beetle cytochrome P450 that hydroxylates myrcene to ipsdienol. Insect Biochem Molec. 2006; 36: 835–845.
- 25. Qiu Y, Tittiger C, Wicker-Thomas C, Le Goff G, Young S, Wajnberg E, et al. An insect-specific P450 oxidative decarbonylase for cuticular hydrocarbon biosynthesis. P Natl Acad Sci USA. 2012; 109: 14858–14863.
- 26. Flück CE, Tajima T, Pandey AV, Arlt W, Okuhara K, Verge CF,et al. Mutant P450 oxidoreductase causes disordered steroidogenesis with and without Antley-Bixler syndrome. Nat Genet. 2004; 36: 228–230. pmid:14758361
- 27. Koener JF. The cDNA and deduced protein sequence of house fly NADPH-cytochrome p450 reductase. Insect Biochem Molec. 1993; 23: 439–447.
- 28. Hovemann B T, Sehlmeyer F, Malz J. Drosophila melanogaster NADPH-cytochrome P450 oxidoreductase: Pronounced expression in antennae may be related to odorant clearance. Gene. 1997; 189: 213–219. pmid:9168130
- 29. Horike N, Takemori H, Nonaka Y, Sonobe H, Okamoto M. Molecular cloning of NADPH-cytochrome P450 oxidoreductase from silkworm eggs: Its involvement in 20-hydroxyecdysone biosynthesis during embryonic development. Eur J Biochem. 2000; 267: 6914–6920. pmid:11082204
- 30. Maïbèche-Coisne M, Merlin C, François MC, Porchero P, Jacquin-Joly E. P450 and P450 reductase cDNAs from the moth Mamestra brassicae: Cloning and expression patterns in male antennae. Gene. 2005; 346: 195–203. pmid:15716002
- 31. Lycett GJ, Mclaughlin LA, Ranson H, Hemingway J, Kafatos FC, Loukeris TG, et al. Anopheles gambiae P450 reductase is highly expressed in oenocytes and in vivo knockdown increases permethrin susceptibility. Insect Mol Biol. 2006; 15: 321–327. pmid:16756551
- 32. Kaewpa D, Boonsuepsakul S, Rongnoparut P. Functional expression of mosquito NADPH-cytochrome P450 reductase in Escherichia coli. J Econ Entomol. 2007; 100: 946–953. pmid:17598560
- 33. Chen XE, Zhang Y. Identification and characterization of NADPH-dependent cytochrome P450 reductase gene and cytochrome b 5 gene from Plutella xylostella: Possible involvement in resistance to beta-cypermethrin. Gene. 2015; 558: 208–214. pmid:25550052
- 34. Tamura K, Peterson D, Peterson N, Stecher G, Nei M, Kumar S. MEGA5: Molecular evolutionary genetics analysis using maximum likelihood, evolutionary distance, and maximum parsimony methods. Mol Biol Evol. 2011; 28: 2731–2739. pmid:21546353
- 35. Kang XL, Zhang M, Wang K, Qiao XF, Chen MH. Molecular cloning and characterization of multidrug resistance protein 1 (MRP1) in the bird cherry-oat aphid, Rhopalosiphum padi (Hemiptera: Aphididae), and the synergistic effects of verapamil. Arch Insect Biochem. 2016.
- 36. Zuo YY, Wang K, Zhang M, Peng X, Pinero JM, Chen MH. Regional susceptibilities of Rhopalosiphum padi (Hemiptera: Aphididae) to ten insecticides. Fla Entomol. 1–18204 R7–87485. 2016.
- 37. Zhang M, Qiao X, Li YT, Fang B, Zuo YY, Chen MH. Cloning of eight Rhopalosiphum padi (Hemiptera: Aphididae) nAChR subunit genes and mutation detection of the β1 subunit in field samples from China. Pestic Biochem Phys.
- 38. Librado P, Rozas J. DnaSP v5: A software for comprehensive analysis of DNA polymorphism data. Bioinformatics. 2009; 25: 1451–1452. pmid:19346325
- 39. Ingelman M, Bianchi V, Eklund H. The three-dimensional structure of flavodoxin reductase from Escherichia coli at 1.7 Å resolution. J Mol Biol. 1997; 268: 147–157. pmid:9149148
- 40. Shen AL, Sem DS, Kasper CB. Mechanistic studies on the reductive half-reaction of NADPH-cytochrome P450 oxidoreductase. J Biol Chem. 1999; 274: 5391–5398. pmid:10026149
- 41. Hubbard PA, Shen AL, Paschke R, Kasper CB, Kim JJP. NADPH-cytochrome P450 oxidoreductase: Structural basis for hydride and electron transfer. J Biol Chem. 2001; 276: 29163–29170. pmid:11371558
- 42. Ramsey JS, Rider DS, Walsh TK, De Vos M, Gordon KHJ, Ponnala L, et al. Comparative analysis of detoxification enzymes in Acyrthosiphon pisum and Myzus persicae. Insect Mol Biol. 2010; 19: 155–164. pmid:20482647
- 43. Li ZQ, Zhang S, Luo JY, Wang CY, Lv LM, Dong SL, et al. Ecological adaption analysis of the cotton aphid (Aphis gossypii) in different phenotypes by transcriptome comparison. PloS one. 2013; 8: e83180. pmid:24376660
- 44. Bass C, Puinean AM, Andrews M, Cutler P, Daniels M, Elias J, et al. Mutation of a nicotinic acetylcholine receptor β subunit is associated with resistance to neonicotinoid insecticides in the aphid Myzus persicae. Bmc Neurosci. 2011; 12: 51. pmid:21627790
- 45. Wang M, Roberts DL, Paschke R, Shea TM, Masters BS, Kim JJ. Three-dimensional structure of NADPH-cytochrome P450 reductase: prototype for FMN- and FAD-containing enzymes. P Natl Acad Sci USA. 1997; 94: 8411–8416.
- 46. Pandey AV, Kempna P, Hofer G, Mullis PE, Flück CE. Modulation of human CYP19A1 activity by mutant NADPH P450 oxidoreductase. Mol Endocrinol. 2007; 21: 2579–2595. pmid:17595315
- 47. Szczesna-Skorupa E, Ahn K, Chen CD, Doray B, Kemper B. The cytoplasmic and N-terminal transmembrane domains of cytochrome P450 contain independent signals for retention in the endoplasmic reticulum. J Biol Chem. 1995; 270: 24327–24333. pmid:7592644
- 48. Lamb DC, Kim Y, Yermalitskaya LV, Yermalitsky VN, Lepesheva GI, Kelly SL, et al. A second FMN binding site in yeast NADPH–cytochrome P450 reductase suggests a mechanism of electron transfer by diflavin reductases. Structure. 2006; 14: 51–61. pmid:16407065
- 49. Murataliev MB, Feyereisen R, Walker FA. Electron transfer by diflavin reductases. BBA-Proteins Proteom. 2004; 1698: 1–26.
- 50. Aigrain L, Fatemi F, Frances O, Lescop E, Truan G. Dynamic control of electron transfers in diflavin reductases. Int J Mol Sci. 2012; 13: 15012–15041. pmid:23203109
- 51. Iyanagi T, Xia C, Kim JJ. NADPH-cytochrome P450 oxidoreductase: Prototypic member of the diflavin reductase family. Arch Biochem Biophys. 2012; 528:72–89. pmid:22982532
- 52. Gilbert LI, Warren JT. A molecular genetic approach to the biosynthesis of the insect steroid molting hormone. Vitam Horm. 2005; 73: 31–57. pmid:16399407
- 53. Petryk A, Warren JT, Marqués G, Jarcho MP, Gilbert LI, Kahler J, et al. Shade is the Drosophila P450 enzyme that mediates the hydroxylation of ecdysone to the steroid insect molting hormone 20-hydroxyecdysone. P Natl Acad Sci USA. 2003; 100: 13773–13778.
- 54. Helvig C, Koener JF, Unnithan GC, Feyereisen R. CYP15A1, the cytochrome P450 that catalyzes epoxidation of methyl farnesoate to juvenile hormone III in cockroach corpora allata. P Natl Acad Sci USA. 2004; 101: 4024–4029.
- 55. Muller P, Warr E, Stevenson BJ, Pignatelli PM, Morgan JC, Steven A, et al. Field-caught permethrin-resistant Anopheles losgambiae overexpress CYP6P3, a P450 that metabolises pyrethroids. Plos Genet. 2008; 4: e1000286. pmid:19043575
- 56. Yang T, Liu N. Genome analysis of cytochrome P450s and their expression profiles in insecticide resistant mosquitoes, Culex quinquefasciatus. Plos One. 2011; 6: e29418. pmid:22242119
- 57. Liu N, Li T, Reid WR, Yang T, Zhang L. Multiple cytochrome P450 genes: Their constitutive overexpression and permethrin induction in insecticide resistant mosquitoes, Culex quinquefasciatus. Plos one. 2011; 6: e23403. pmid:21858101
- 58. Liu N, Li M, Gong Y, Liu F, Li T. Cytochrome P450s–Their expression, regulation, and role in insecticide resistance. Pestic Biochem Phys. 2015; 120: 77–81.
- 59. Carino FA, Koener JF, Plapp FW, Feyereisen R. Constitutive overexpression of the cytochrome P450 gene CYP6A1 in a house fly strain with metabolic resistance to insecticides. Insect Biochem Molec. 1994; 24: 411–418.
- 60. Silva AX, Jander G, Samaniego H, Ramsey JS, Figueroa CC. Insecticide resistance mechanisms in the green peach aphid Myzus persicae (Hemiptera: Aphididae) I: A transcriptomic survey. Plos One. 2012; 7: e36366. pmid:22685538
- 61. Silva AX, Bacigalupe LD, Luna-Rudloff M, Figueroa CC. Insecticide resistance mechanisms in the green peach aphid Myzus persicae (Hemiptera: Aphididae) II: Costs and benefits. Plos one. 2012; 7: e36810. pmid:22685539
- 62. Aliferis KA, Jabaji S. Metabolomics–A robust bioanalytical approach for the discovery of the modes-of-action of pesticides: A review. Pestic Biochem Phys. 2011; 100: 105–117.
- 63. Zhao C, Tang T, Feng X, Qiu L. Cloning and characterisation of NADPH-dependent cytochrome P450 reductase gene in the cotton bollworm, Helicoverpa armigera. Pest Manag Sci. 2014; 70: 130–139. pmid:23512641
- 64. Sarapusit S, Xia C, Misra I, Rongnoparut P, Kim JJP. NADPH-cytochrome P450 oxidoreductase from the mosquito Anopheles minimus: Kinetic studies and the influence of Leu86 and Leu219 on cofactor binding and protein stability. Arch Biochem Biophy. 2008; 477: 53–59.
- 65. Sarapusit S, Lertkiatmongkol P, Duangkaew P, Rongnoparut P. Modeling of Anopheles minimus mosquito NADPH-cytochrome P450 oxidoreductase (CYPOR) and mutagenesis analysis. Int J Mol Sci. 2013; 14: 1788–1801. pmid:23325047
- 66. Marohnic CC, Spmccammon P. Human cytochrome P450 oxidoreductase deficiency caused by the Y181D mutation: Molecular consequences and rescue of defect. Drug Metab Dispos. 2010; 38: 332–340. pmid:19884324
- 67. Xia C, Panda SP, Marohnic CC, Martasek P, Masters BS, Kim JJ. Structural basis for human NADPH-cytochrome P450 oxidoreductase deficiency. Proc Natl Acad Sci USA. 2011; 108:13486–13491. pmid:21808038
- 68. Marohnic CC, Martásek PS, Masters BS. Diminished FAD binding in the Y459H and V492E Antley-Bixler syndrome mutants of human cytochrome P450 reductase. J Biol Chem. 2006; 281:35975–35982. pmid:16998238
- 69. Huang N, Agrawal V, Giacomini KM, Miller WL. Genetics of P450 oxidoreductase: Sequence variation in 842 individuals of four ethnicities and activities of 15 missense mutations. Proc Natl Acad Sci USA. 2008; 105: 1733–1738. pmid:18230729