Chemosensory Gene Families in the Oligophagous Pear Pest Cacopsylla chinensis (Hemiptera: Psyllidae)

Chemosensory systems play an important role in insect behavior, and some key associated genes have potential as novel targets for pest control. Cacopsylla chinensis is an oligophagous pest and has become one of the main pests of pear trees, but little is known about the molecular-level means by which it locates its hosts. In this study, we assembled the head transcriptome of C. chinensis using Illumina sequencing, and 63,052 Unigenes were identified. A total of 36 candidate chemosensory genes were identified, including five different families: 12 odorant binding proteins (OBPs), 11 chemosensory proteins (CSPs), 7 odorant receptors (ORs), 4 ionotropic receptors (IRs), and 2 gustatory receptors (GRs). The number of chemosensory gene families is consistent with that found in other Hemipteran species, indicating that our approach successfully obtained the chemosensory genes of C. chinensis. The tissue expression of all genes using quantitative real-time PCR (qRT-PCR) found that some genes displayed male head, female head, or nymph-biased specific/expression. Our results enrich the gene inventory of C. chinensis and provide valuable resources for the analysis of the functions of some key genes. This will help in developing molecular targets for disrupting feeding behavior in C. chinensis.


Introduction
Insect chemosensory systems interpret and react to various environmental chemical factors, and impact various life cycle processes, including feeding, predator avoidance, and reproductive behavior [1,2]. Recognition of these behaviors frequently involves a series of genes, including those that encode odorant binding proteins (OBPs), chemosensory proteins (CSPs), odorant receptors (ORs), ionotropic receptors (IRs), and gustatory receptors (GRs) [3][4][5]. These proteins participate in extremely complex biochemical reactions in various tissues to ensure accurate delivery of chemical signals [6].
OBPs and CSPs are two families of integral membrane proteins located on the dendrites of olfactory receptor neurons (ORNs), and are abundant in the lymph antennae [7]. These can capture and

Tissue Sample Collection
The morphological picture of C. chinensis is shown in Figure 1. Three hundred C. chinensis (100 males, 100 females, and 100 nymphs) were collected from Dangshan (34 • 27'42.62" N, 116 • 31'40.72" E), Suzhou, China. The 300 heads were dissected out under a stereomicroscope with a sterile scalpel and immediately mixed into liquid nitrogen and sent to Genepioneer Biotech Corporation (Nanjing, China) for RNA-seq. For quantitative real-time PCR (qRT-PCR) analysis, we separately collected 60 males, 60 females, and 60 nymphs divided into heads only or bodies only. They were separately named as MH, male head; MB, male body; FH, female head; FB, female body; NH, nymph head and NB, nymph body and placed in nuclease-free centrifuge tubes as one replicate. Each replicate was repeated three times. All samples were preserved in liquid nitrogen until RNA extraction.

Total RNA Extraction and cDNA Synthesis
We used the MiniBEST Universal RNA Extraction Kit (TaKaRa, Dalian, China) to extract total RNA following the manufacturer's instructions. RNA quality and concentration were analyzed using an ultramicro-spectrophotometer (MD2000D, Biofuture, UK). The RNA was stored at -80 °C prior to use. Single-stranded cDNA templates were synthesized using 1 μg total RNA from various tissue samples, using primers from the PrimeScript TM RT Master Mix (TaKaRa, Dalian, China).

Library Preparation for Transcriptome Sequencing
For sequencing, total RNA was extracted using the TRIzol ® reagent (Tiangen Biotech, Beijing, China) [44,45] and checked for quality. The mRNA was enriched using magnetic beads, then fragmented randomly by adding fragmentation buffer. First-strand cDNA was synthesized using mRNA templates and a random hexamer and the second cDNA chain was synthesized by adding buffers, dNTPs, RNAse H, and DNA polymerase I. The cDNA was then purified using AMPure XP beads (Beckman Coulter, Beverly, MA, USA). Purified double-strand cDNA was used for end repair, adding poly-A tails and adapters [46]. Finally, cDNA libraries were obtained by PCR. Library concentration and insert size were detected using a Qubit ® 2.0 Fluorometer (Life Technologies, Grand Island, NY, USA) and an Agilent Bioanalyzer 2100 system. Quantitative qRT-PCR was used to accurately quantify the effective concentration of the library to ensure its quality. Finally, the cDNA library was sequenced using an Illumina Hiseq 4000 platform with the paired-end (PE) and the sequencing read length was PE150bp.

De Novo Assembly and Unigene Annotation
After using sequencing by synthesis (SBS) technology, raw reads were cleaned by removing adaptor reads, ambiguous reads ('N' > 10%), and low-quality reads (that is, where more than 50% of bases in a read had a quality value Q ≤ 5) using Perl script. Clean reads were then de novo assembled

Total RNA Extraction and cDNA Synthesis
We used the MiniBEST Universal RNA Extraction Kit (TaKaRa, Dalian, China) to extract total RNA following the manufacturer's instructions. RNA quality and concentration were analyzed using an ultramicro-spectrophotometer (MD2000D, Biofuture, UK). The RNA was stored at −80 • C prior to use. Single-stranded cDNA templates were synthesized using 1 µg total RNA from various tissue samples, using primers from the PrimeScript TM RT Master Mix (TaKaRa, Dalian, China).

Library Preparation for Transcriptome Sequencing
For sequencing, total RNA was extracted using the TRIzol ® reagent (Tiangen Biotech, Beijing, China) [44,45] and checked for quality. The mRNA was enriched using magnetic beads, then fragmented randomly by adding fragmentation buffer. First-strand cDNA was synthesized using mRNA templates and a random hexamer and the second cDNA chain was synthesized by adding buffers, dNTPs, RNAse H, and DNA polymerase I. The cDNA was then purified using AMPure XP beads (Beckman Coulter, Beverly, MA, USA). Purified double-strand cDNA was used for end repair, adding poly-A tails and adapters [46]. Finally, cDNA libraries were obtained by PCR. Library concentration and insert size were detected using a Qubit ® 2.0 Fluorometer (Life Technologies, Grand Island, NY, USA) and an Agilent Bioanalyzer 2100 system. Quantitative qRT-PCR was used to accurately quantify the effective concentration of the library to ensure its quality. Finally, the cDNA library was sequenced using an Illumina Hiseq 4000 platform with the paired-end (PE) and the sequencing read length was PE150bp.

De Novo Assembly and Unigene Annotation
After using sequencing by synthesis (SBS) technology, raw reads were cleaned by removing adaptor reads, ambiguous reads ('N' > 10%), and low-quality reads (that is, where more than 50% of bases in a read had a quality value Q ≤ 5) using Perl script. Clean reads were then de novo assembled using the Trinity program v2.4.0 (http://trinityrnaseq.sourceforge.net/) with default parameters [47], and the minimal contig length is 301 bp. The reads of C. chinensis have been deposited (accession number: SRA9127897). BLAST (http://blast.ncbi.nlm.nih.gov/Blast.cgi) was used to compare Unigene sequences with databases including Nr (non-redundant database) [48], Swiss-Prot [49], KEGG (Kyoto Encyclopedia of Genes and Genomes) [50], KOG (EuKaryotic Orthologous Groups) [51], and COG (Clusters of Orthologous Groups) [52] to obtain amino acid sequences of Unigene genes. Then, HMMER [53] software was used to compare with the Pfam [54] database (including chemosensory proteins families in different insects) to obtain the annotation information of Unigene.

Phylogenetic Analysis
Phylogenetic trees were constructed using amino acid sequences of candidate genes including CchiOBPs, CchiCSPs, CchiORs, CchiIRs, and CchiGRs of C. chinensis (Table S1), and the signal peptide sequences of OBPs and CSPs were predicted by SignalP 4.1 server [55] with default parameters and then removed. The sequences were aligned by using ClustalX 2.0 (University College Dublin, Dublin, Ireland), and phylogenetic trees were constructed using PhyML [56] based on an LG substitution model [57] with nearest-neighbor interchange (NNI). Branch support was estimated using a Bayesian-like transformation of the aLRT (aBayes) method. Dendrograms were edited using FigTree software (http://tree.bio.ed.ac.uk/software/figtree/).

Quantitative Real-Time PCR
We used qRT-PCR to determine the relative expression levels of chemosensory genes in different tissues (MH, MB, FH, FB, NH, and NB). The experiment was performed in a LightCycler ® 96 (Roche Diagnostics Gmbh, Basel, Switzerland) according to the minimum information for publication of qRT-PCR experiments [58], using a total mixture of 10 µL with 5 µL 2X SYBR Green PCR Master Mix (YIFEIXUE BIO TECH, Nanjing, China), 0.2 µL paired primers designed using Beacon Designer 7.9 (PREMIER Biosoft International, CA, USA) (Table S2) to check for the absence of primer-dimer peaks, 3.6 µL nuclease-free water, and 1 µL cDNA. The amplification step was executed using a degeneration step at 95 • C for 10 min, followed by 40 cycles of 95 • C for 15 s and 60 • C for 60 s. The melting curve detected a single primer-specific peak, using 93 • C for 30 s and 60 • C for 45 s. A negative control was created using distilled water instead of cDNA template for each test run.
CchiGAPDH (glyceraldehyde-3-phosphate dehydrogenase) and CchiEF (elongation factor 1-alpha) (Genbank numbers CchiGAPDH: MK940861, CchiEF: MK940862) were used as internal reference genes to calculate the expression of different genes in different tissues. This was carried out using the Microsoft Excel-based software Visual Basic using the Q-Gene method [59]. For six samples, each biological sample was repeated three times in a LightCycler ® 96 multiwell plate.

Statistical Analysis
Relative expressions of chemosensory genes (mean ± standard error) were compared using one-way ANOVA in SPSS 21.0 software (SPSS Inc., Chicago, IL, USA), according to the least significance difference (LSD). Differences were regarded as significant at p < 0.05. The GraphPad TM Prism 7.0 software (GraphPad Software Inc., San Diego, CA, USA) was used to perform the figures [60].

Transcriptome Sequencing and Assembly
We generated a total of 32,879,148 clean reads from a cDNA library using transcriptome sequencing ( Table 1). The percentage of reads with Q20 and Q30 quality scores was 99% and 91.25%, respectively. De novo assembly yielded 63,052 Unigenes of high assembly integrity with a mean length of 64,826 bp and a maximum length of 20,509 bp.

Odorant Binding Proteins (OBPs)
A total of twelve putative OBP genes were identified and named as CchiOBP1-12. The phylogenetic trees of the CchiOBPs were constructed using three Hemipteran species, including D. citri, Aphis gossypii, Sogatella furcifera, and Diptera Drosophila melanogaster ( Figure 3). The results show that CchiOBPs had several putative one-to-one orthologous relationships with these species, and only CchiOBP1 belongs to the Plus-C subgroup; the other CchiOBPs were clustered in the Classic subgroup. Among the CchiOBP genes, six CchiOBPs (CchiOBP1, CchiOBP4, CchiOBP5, CchiOBP9, CchiOBP10, and CchiOBP12) had full open reading frames (ORFs) to encode 104 to 238 amino acids and had signal peptides at the N-terminus ( Table 2). The expression profiles of all CchiOBPs showed Species that have more than 3% matching hits to the C. chinensis transcripts are shown.

Odorant Binding Proteins (OBPs)
A total of twelve putative OBP genes were identified and named as CchiOBP1-12. The phylogenetic trees of the CchiOBPs were constructed using three Hemipteran species, including D. citri, Aphis gossypii, Sogatella furcifera, and Diptera Drosophila melanogaster (Figure 3). The results show that CchiOBPs had several putative one-to-one orthologous relationships with these species, and only CchiOBP1 belongs to the Plus-C subgroup; the other CchiOBPs were clustered in the Classic subgroup. Among the CchiOBP genes, six CchiOBPs (CchiOBP1, CchiOBP4, CchiOBP5, CchiOBP9, CchiOBP10, and CchiOBP12) had full open reading frames (ORFs) to encode 104 to 238 amino acids and had signal peptides at the N-terminus ( Table 2). The expression profiles of all CchiOBPs showed that all CchiOBPs were highly expressed in the heads (Figure 4). Among the CchiOBPs, five CchiOBPs (CchiOBP1, 3-6) were more highly expressed in female heads (FH) than in male heads (MH) (p < 0.05). CchiOBP12 was highly expressed in the heads of both male and female adults. Three CchiOBPs (CchiOBP7, CchiOBP10, and CchiOBP11) were highly expressed in male heads, with CchiOBP7 exhibiting the highest expression level. Additionally, two CchiOBPs (CchiOBP2 and 9) exhibited significantly higher expression in nymph heads (NH) than other tissues, and CchiOBP8 showed specific expression in nymphs.
Insects 2019, 10, x 6 of 20 (CchiOBP7, CchiOBP10, and CchiOBP11) were highly expressed in male heads, with CchiOBP7 exhibiting the highest expression level. Additionally, two CchiOBPs (CchiOBP2 and 9) exhibited significantly higher expression in nymph heads (NH) than other tissues, and CchiOBP8 showed specific expression in nymphs.

Chemosensory Proteins (CSPs)
In all, we identified eleven transcripts encoding putative CSPs in C. chinensis. Seven were full-length genes with predicted signal peptide sequences (Table 2) and had four conserved cysteines in corresponding positions. All CchiCSPs shared 37-89% amino acid identity with other Hemipteran insects. The phylogenetic tree results indicate that all CchiCSPs were distributed on various branches, with one D. citri ortholog distribution on each branch ( Figure 5). The qRT-PCR results of all CchiCSPs showed that CchiCSP1, CchiCSP3, and CchiCSP8 were highly or specifically expressed in nymph heads. CchiCSP2 had adult head-biased expression, but CchiCSP4 displayed adult body-specific expression. CchiCSP9 and CchiCSP10 were significantly highly expressed in male and female bodies, respectively ( Figure 6).

Chemosensory Proteins (CSPs)
In all, we identified eleven transcripts encoding putative CSPs in C. chinensis. Seven were fulllength genes with predicted signal peptide sequences (Table 2) and had four conserved cysteines in corresponding positions. All CchiCSPs shared 37-89% amino acid identity with other Hemipteran insects. The phylogenetic tree results indicate that all CchiCSPs were distributed on various branches, with one D. citri ortholog distribution on each branch ( Figure 5). The qRT-PCR results of all CchiCSPs showed that CchiCSP1, CchiCSP3, and CchiCSP8 were highly or specifically expressed in nymph heads. CchiCSP2 had adult head-biased expression, but CchiCSP4 displayed adult body-specific expression. CchiCSP9 and CchiCSP10 were significantly highly expressed in male and female bodies, respectively ( Figure 6).

Odorant receptors (ORs), ionotropic receptors (IRs), and gustatory receptors (GRs)
We identified 13 distinct Unigenes putatively as seven ORs, four IRs, and two GRs ( Table 2). Phylogenetic trees for CchiORs (Figure 7), CchiIRs (Figure 8), and CchiGRs ( Figure 9) were constructed using amino acid sequences from C. chinensis and other insects. We found that the CchiORs were highly homologous to D. citri, and CchiOR2 belonged to the Orco family that is widely expressed and highly conserved in insects. In the phylogenetic tree of CchiIRs and CchiGRs, we found that all CchiIRs belong to the antennal IRs, but CchiGRs were not clustered in the CO2 or sugar receptor families. Tissue expression analysis showed that almost all were more highly expressed in

Odorant receptors (ORs), ionotropic receptors (IRs), and gustatory receptors (GRs)
We identified 13 distinct Unigenes putatively as seven ORs, four IRs, and two GRs ( Table 2). Phylogenetic trees for CchiORs (Figure 7), CchiIRs (Figure 8), and CchiGRs ( Figure 9) were constructed using amino acid sequences from C. chinensis and other insects. We found that the CchiORs were highly homologous to D. citri, and CchiOR2 belonged to the Orco family that is widely expressed and highly conserved in insects. In the phylogenetic tree of CchiIRs and CchiGRs, we found that all CchiIRs belong to the antennal IRs, but CchiGRs were not clustered in the CO 2 or sugar receptor families. Tissue expression analysis showed that almost all were more highly expressed in adults than in nymphs, although CchiOR6 was specifically expressed in the male bodies of nymphs ( Figure 10). CchiOR1 and CchiOR2 were more highly expressed in adult heads compared to other tissues, and CchiOR3 and CchiOR4 were more expressed in male heads and bodies. Meanwhile, CchiOR5 was more abundant in nymph and female heads. CchiIR1 and CchiIR3 were more highly expressed in nymph bodies and female bodies, respectively, while CchiIR2 showed adult head-biased expression. However, both CchiGR1 and CchiGR2 were highly expressed in nymph heads ( Figure 10). adults than in nymphs, although CchiOR6 was specifically expressed in the male bodies of nymphs ( Figure 6). CchiOR1 and CchiOR2 were more highly expressed in adult heads compared to other tissues, and CchiOR3 and CchiOR4 were more expressed in male heads and bodies. Meanwhile, CchiOR5 was more abundant in nymph and female heads. CchiIR1 and CchiIR3 were more highly expressed in nymph bodies and female bodies, respectively, while CchiIR2 showed adult head-biased expression. However, both CchiGR1 and CchiGR2 were highly expressed in nymph heads ( Figure 6).

Discussion
As an important olfactory and taste organ, insect heads are important in communication and feeding behavior [61]. Therefore, the head has always been important in insect research, and a certain number of chemosensory genes have been found in the heads of different insects, such as S. furcifera [61], Tomicus yunnanensis [62], and Mythimna separate [63]. This suggests that chemosensory genes in

Discussion
As an important olfactory and taste organ, insect heads are important in communication and feeding behavior [61]. Therefore, the head has always been important in insect research, and a certain number of chemosensory genes have been found in the heads of different insects, such as S. furcifera [61], Tomicus yunnanensis [62], and Mythimna separate [63]. This suggests that chemosensory genes in insect heads should be associated with the above-mentioned chemosensory behaviors. In this study, we first sequenced and analyzed the head transcriptome of C. chinensis, and identified 36 chemosensory genes (12 OBPs,11 CSPs,7 ORs, 4 IRs, and 2 GRs), indicating C. chinensis can also regulate the corresponding behavioral response with the chemosensory genes of the head, just like the insects mentioned above. However, the number of chemosensory genes of C. chinensis is less than that of other Hemipteran insects, including 9 OBPs, 9 CSPs, 45 ORs, and 14 IRs of A. gossypii [64,65]; 9 OBPs, 12 CSPs, 46 ORs, 35 IRs, and 20 GRs of D. citri [66]; 12 OBPs, 9 CSPs, 63 ORs, and 14 IRs of S. furcifera [67,68]; and 11 OBPs, 17 CSPs, 50 ORs, and 10 GRs of Nilaparvata lugens [69,70]. This may reflect the fact that C. chinensis is an oligophagous insect and does not need as many chemosensory genes to recognize host volatiles.
The tissue expression results showed that all CchiOBPs were highly expressed in heads, indicating their involvement in the olfactory and gustatory processes of C. chinensis. Among the CchiOBPs, five CchiOBPs (CchiOBP1, 3-6) and two CchiOBPs (CchiOBP7, 11) were significantly highly expressed in the heads of females and males, respectively. Previous studies have revealed the different functions of OBPs in the chemosensory organs of insect heads. Female mosquitoes of Culex quinquefasciatus use CquiOBP1 to detect oviposition attractants [71,72], and male moths of Spodoptera litura recognize the female sex pheromones by pheromone binding proteins (SlitPBPs) [73], suggesting that insect OBPs participate in sex-related chemosensory behavior, and the seven CchiOBPs may have similar functions, i.e., regulating oviposition or mating behavior by detecting different pear volatiles or intraspecific pheromones. Additionally, two CchiOBPs (CchiOBP2 and 9) were significantly highly expressed in nymph heads. The highly expressed NlugOBP3 in nymphs of N. lugens is involved in nymph olfaction on rice seedlings as determined by integrating RNAi and ligand binding assays [74]. Thus, the two CchiOBPs may help C. chinensis to complete the feeding process on pear trees by detecting the pear volatiles. Interestingly, we found that CchiOBP8 was specifically expressed in both nymph heads and bodies, suggesting that it may take part in the feeding and/or other physiological processes of nymphs. The OBP phylogenetic tree showed that most CchiOBPs were adjacent in the phylogenetic tree to DcitOBPs of D. citri, indicating that the two species have high homology and some OBPs might have similar functions. The CchiOBP1 was clustered into the plus-C OBP subfamily, and others belonged to the classic subfamily, which is similar to D. citri and S. furcifera [66,68], suggesting that the mechanism of functional differentiation of OBPs in Hemiptera insects may be the same.
Among all CchiCSPs, six CchiCSPs displayed head-biased expression, suggesting that these genes may have similar functions to the high expression of CchiOBPs in the head. The functions of CSPs expressed in important chemosensory organs of the head have been reported in different insects, such as SfurCSP5 of S. furcifera has high affinities for three rice volatiles (2-tridecanone, 2-pentadecanone, and β-ionone) [75], and three host volatiles [(Z)-3-hexen-1-ol, (E)-2-hexen-1-al, and valeraldehyde] have a high binding affinity with AlinCSPs (1, 2, and 3) of A. lineolatus [76], and SinfCSP19 of Sesamia inferens is able to bind sex pheromones and host plant volatiles [77]. These results suggest that this type of insect CSP may have similar functions as OBP in recognizing host volatiles and sex pheromones. In addition, many insect CSPs are broadly expressed in different tissues (leg, gut, and pheromone gland) [78][79][80][81][82][83] and have non-chemosensory functions; for example, SexiCSP3 is involved in survival and reproduction in S. exigua [84], AmelCSP5 is crucial in the formation of embryonic integument in Apis mellifera [85], and some midgut-expressed SlitCSPs of S. litura may have functional roles in the specialization and adaption to different ecosystems [82]. In our study, five of 11 CchiCSPs in C. chinensis were widely expressed in all investigated tissues, suggesting that these CchiCSPs may be involved in governing host plant choice and other physiological behaviors. According to our phylogenetic tree of CchiCSP genes, CSPs from C. chinensis and D. citri were grouped in the same clade, indicating that some CSP genes may have similar functions between the two species.
Chemosensory receptors stimulate corresponding physiological behavior of insects [86][87][88], and identification of chemosensory receptors is a key step in interpreting mechanisms of insect chemosensation. In this study, the OR phylogenetic trees showed that CchiOR2 belongs to the Orco family, which is necessary for locating other conventional ORs on dendritic membranes and for odor detection [89], and which indicates that C. chinensis shares chemosensory mechanisms with other insects [90,91]. Seven of 13 chemosensory receptor genes were highly expressed in the heads. Among them, two conventional CchiORs (CchiOR1 and 4) were more abundant in male heads than in other tissues, indicating that they may participate in recognizing odorants such as pheromones related to male physiological activities. This is similar to the pheromone receptor (PR) of moths, which specializes in the recognition of female sex pheromones [7,92,93]. Previous studies revealed a female-biased AlucOR46 of Apolygus lucorum tunes to some plant volatiles [(S)-(−)-limonene, (R)-(+)-limonene, (E)-2-hexenal, (E)-3-hexenol, 1-heptanol, and (1R)-(−)-myrtenol)] [94], three female-biased ORs of B. mori (OR19, 45 and 47) account for some of the female-specific odorant responses, such as oviposition cues (plant volatiles: linalool, benzoic acid, 2-phenylethanol and benzaldehyde) and/or detection of an as yet unidentified male-produced sex pheromone [95,96], and larvae-expressed BmorOR56 has high selective tuning to cis-jasmone, a key mulberry leaf volatile [97]. Thus, CchiOR5, which was highly expressed in both female and nymph heads, may have similar roles in C. chinensis. Mang found that larvae-expressed BmorGR9 is involved in the promotion of feeding behaviors [98], indicating that CchiGR1 and 2, which were highly expressed in nymph heads, may also participate in the feeding progress of C. chinensis. BmorGR6, which exists in different tissues (midgut, central nervous system, and oral sensory organs), is not only a taste receptor but also a chemical sensor for the regulation of gut movement, physiological conditions, and feeding behavior of B. mori larvae [99]. The highly expressed foregut-specific HarmGR9 of H. armigera may contribute to the regulation of larval feeding behavior [100], and some SlitIRs of S. litura were detected in proboscises, legs, abdomens, and reproductive tissues and may have diverse functional roles in olfaction, taste, and reproduction [101]. We also found widely-expressed genes such as CchiOR7 and CchiIR4, in contrast to those highly or specifically expressed in female and/or nymph bodies (CchiIR3, CchiIR1, and CchiOR6), indicating these five chemosensory receptors may play a vital role in regulating feeding and other physiological behaviors. The exact function of these genes could be further analyzed by integrating in vivo and in vivo methods [92,93,102].

Conclusions
In conclusion, we identified an extensive set of chemosensory genes that may be related to the chemosensory and gustatory behaviors of C. chinensis by sequencing and analyzing head transcriptomic data. As a first step towards understanding their functions, we comprehensively compared phylogeny and tissue expression and demonstrated male head, female head, and nymph-biased specific/expression genes. Our results provide a valuable resource for analyzing the function of key genes in developing effective biological control agents, as well as helping to describe the chemosensory system in C. chinensis and other oligophagous pests.

Conflicts of Interest:
The authors declare no conflict of interest.