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A Gustatory Receptor Used for Rapid Detection of Tyrophagus putrescentiae in Fungi Hosts


The storage mite, Tyrophagus putrescentiae, found worldwide in many habitats, is an important pest of edible fungi in China. Storage mites are tiny and difficult to observe, especially when they occur in fungi composts. In this study, one gustatory receptor protein (TputGR1) was identified from the transcriptome of T. putrescentiae. Phylogenetic analysis of GRs families from 10 arthropod species revealed that TputGR1 had high homology with the SccaGR1 of Sarcoptes scabiei and TurtGR1-2 of Tetranychus urticae, but low homology with other insect species, Drosophila melanogaster, Anopheles gambiae, Bombyx mori, Aedes aegypti, Culex quinquefasciatus, and Pediculus humanus. We developed a detection system for the mite on fungi hosts using the GR protein and the loop-mediated isothermal amplification (LAMP). This procedure was rapid (60 min from sampling to result) and had high sensitivity (0.5 ng/mL). LAMP provided rapid and reliable detection of T. putrescentiae. It has good specificity for single samples and for large-scale surveys.


The storage mite, Tyrophagus putrescentiae, is one of the most common synanthropic mites. It has a wide range of habitats, including stored products, crop seeds, mushrooms, foods of domestic animals and pets, and house dust1. It also causes human allergic dermatitis2, pulmonary acariasis and intestinal acariasis3. Fungi have large amounts of nitrogen and phosphorus and produce vitamins and sterols, which are important for mite development4. Fungi also produce exoenzymes, which can enhance utilization of predigested substrates by mites5,6. T. putrescentiae feeds on fungi mycelia and fruit bodies and increases fungi transmission7. As so, it is a pest of mycology laboratories and edible fungi cultivation8,9. Storage mites are too small (adult body length, 280–420 μm) to easily observe and their effects are often mistaken for diseases10.

Mites can disperse by wind (anemochory) or hitchhike on animals (phoresy). Mites in the phoretic stage must possess sensory capabilities needed for locating and identifying potential insect hosts. Once a potential host is found, they must have the mechanical ability to climb on and attach to the host insect11. However, the sensory capabilities of mites are virtually unknown12. Animals use semiochemicals or pheromones to communicate, and then have a series of behavioral responses, such as feeding, mating, avoidance, marking territory, finding prey, and host recognition13,14. In this process, several important chemosensory gene families are involved, including odorant binding proteins (OBPs), chemosensory proteins (CSPs), pheromone binding protein (PBPs), odorant degrading enzymes (ODEs) and chemical receptors, such as odorant (ORs), ionotropic (IRs) and gustatory receptors (GRs)15. Research on the molecular mechanism of chemoreception has demonstrated that volatile chemicals activate a single class of sensory neurons, which target the glomerulus and connect to projection neurons that respond exclusively to the chemicals16.

In this study, the GRs family was identified for the first time in T. putrescentiae by transcriptome sequencing. The GR genes were used for rapid detection of the storage mite from sample materials including bacteria, host fungi, competitive fungi, and fungus gnats using loop-mediated isothermal amplification (LMAP). LAMP of DNA is an alternative to PCR-based methods in food safety testing17 and a variety of other applications including detection of plant diseases and viruses in animals and plants18,19,20. Its advantages over PCR-based techniques include shorter reaction time, no need for specific equipment, high sensitivity and specificity, and comparably low susceptibility to inhibitors present in sample materials. This enables detection of the pathogens in sample materials without lengthy sample preparation.


Identification of GR genes from T. putrescentiae transcriptome

A total of 84,756 unigenes with a mean length of 684 nt were assembled from about 48.91 million clean reads and 51.53 million raw reads (Table 1) by Illumina HiSeq2000. A total of 9,408 unigenes (11.10%) were larger than 1,000 nt in length. Of these genes, 38,169 unigenes (45.03%) were annotated in the NCBI NR database (e-value < 1e-5).

Table 1 The primers used in the LAMP assay.

Gene ontology (GO) annotation of the unigenes was obtained using Blast2GO pipeline and a blastx search against NR. A total of 39,127 unigenes were assigned GO terms. In the biological process terms, the genes were mostly enriched in cellular and metabolic processes. In molecular function terms, molecular binding activity and catalytic activity were the most represented. In cellular component terms, cell, cell part, organelle, organelle part, macromolecular, membrane and membrane part were the most abundant (Fig. 1).

Figure 1

Gene Ontology classifications of the T. putrescentiae unigenes.

The unigenes related to gustatory receptors (GRs) were identified by keyword search of annotations in the seven databases. We identified distinct unigenes encoding one putative GR, and it was named TputGR1 following nomenclature previously established for T. putrescentiae21.

Sequence analysis and phylogenetic tree construction

Sequence analysis confirmed the new one GR, TputGR1, as a 1330-bp long full-length transcript. TputGR1 had high homology with SccaGR1 of Sarcoptes scabiei and TurtGR1-2 of Tetranychus urticae, but low homology with other insect species (Fig. 2). Almost all GRs in Acari were orthologous with insects in the phylogenetic tree. Some GRs with related multi-functions were clustered into the same subgroup including 12 CO2 receptors in insects (including BmorGR11 and 24, AgamGR22, 23 and 24, DmelGR63a, AaegGR1-3 and CquiGR1-3)22,23, and 33 sugar receptors in insects (DmelGR5a, 61a, 64a-d and 64 f, BmorGR8 and 64a, AgamGR14-18 and 20-21, AaegGR5-6 and 8-10 and CquiGR7a, 5-15 and 17)22,24,25. No orthologs were found for 42 of the 54 GRs of Metaseiulus occidentalis and these were clustered into one subgroup. The remaining 11 of the 54 GRs of M. occidentalis were clustered together with all 21 GRs of Ixodes scapularis (Fig. 2). The expansion and diversification of the tick and mite GRs probably reflected the diverse evolutionary histories of chemosensory receptors in the Acari.

Figure 2

Unrooted phylogenetic tree of GR protein sequences from T. putrescentiae (red branches), Drosophila melanogaster (green branches), Anopheles gambiae (yellow branches), Bombyx mori (pink branches), Aedes aegypti (skyblue branches), Culex quinquefasciatus (chocolate branches), I. scapularis (brown branches), M. occidentalis (orange branches), S. scabiei (gray branches), T. urticae (olive branches) and Pediculus humanus (purple branches). Outer ring indicates the different groups and protein functions.

Development of the loop-mediated isothermal amplification detection system

We developed of the loop-mediated isothermal amplification involved primer combinations with a high sensitivity and no false positives. A set of primers suitable for LAMP detection of T. putrescentiae (TP) was designated by F3-Gr09, B3-Gr09, FIP-Gr09, and BIP -Gr09 (Table 0). FIP-Gr09 and BIP -Gr09 were labeled with FAM and biotin, respectively. Primer combination, F3-Gr09, B3-Gr09, FIP-Gr09, and BIP -Gr09 gave a high sensitivity with no false positives and gel electrophoresis results below the strip graph confirmed the LAMP reaction corresponding to the results on the strip (Fig. 3B). The amplification of TputGR1 by LAMP produced a ladder-like pattern, whereas the PCR product was a specific DNA band. Agarose gel electrophoresis analysis indicated that the LAMP reaction did not detect the mushroom mites, Rhizoglyphus robini and Mahunkania secunda, the fungus gnat, Bradysia difformis, the mushroom pathogen, Pseudomonas tolaasii, and the mycelia of Pleurotus ostreatus host (all samples called TPDV). In addition to gel electrophoresis, both visual inspection and strip graph were performed to detect positive reactions and validate the LAMP results. Upon addition of the SYBR green I dye to tubes after the LAMP reaction, the color changed to yellowish green in the positive reactions (Fig. 3A). Similar results were found in the lateral flow strip detection (Fig. 3B).

Figure 3

Correlation of color change and gel electrophoresis of the amplification LAMP results. The positive result produced yellowish green color in (A), two bands in (B) and a ladder-like pattern in (C). Samples 1–6 are Tyrophagus putrescentiae, Rhizoglyphus robini, Bradysia difformis, Mahunkania secunda, Pleurotus ostreatus and Pseudomonas tolaasii, respectively.

Optimization of loop-mediated isothermal amplification (LAMP)

LAMP assay optimizations focused on reaction temperature, reaction time and DNA concentration. A reaction temperature of 60 °C was selected for the LAMP assays (Fig. 4A), similar to a previous report26. The reaction time was extended by 10 and 20 min based on optimum experimental conditions to determine the relationship between reaction time and sensitivity. When LAMP reactions were incubated for 60 min, favorable results were obtained without nonspecific amplification (Fig. 4B). The sensitivity of LAMP was higher than that under 60 min (Fig. 4B). In addition, amplification results from the optimized LAMP assay correlated 100% with results on gel electrophoresis.

Figure 4

Optimization of LAMP. (A) LAMP with 58, 60, 62 or 65 °C of reaction temperature. (B) LAMP with 20, 30, 40, 50 or 60 min of reaction time. (C) LAMP with 50, 10, 1.0, 0.5, 0.3 or 0.15 ng/μL of TP target. The results of the color change were also verified by gel electrophoresis (down) and lateral flow strip detection (up, 2).

The total volume for the LAMP amplification was 25 μL. The optimal concentration of each reagent was as follows: F3-Gr09, 0.1 μM; B3-Gr09, 0.1 μM; FIP-Gr09, 0.4 μM; BIP-Gr09, 0.4 μM; MgSO4, 0.5 mM; dNTP, 0.24 mM; and 1 × Bst DNA polymerase buffer and Bst DNA polymerase (8 U/μL), 2 μL. The assay could detect TP containing DNA target (50 ng/μL) at 10−1 dilution after 60 min amplification.

Evaluation and validation of LAMP-TP with clinical specimens

A total of 37 samples from swine suspected of having TP infections were collected from Chengdu (Agaricus bisporus host), Harbin (Flammulina velutipes host), and Jinan (P. ostreatus host). The samples were tested for validation of the LAMP-TP in TP detection. A no template control and three uninfected hosts, P. ostreatus (PO), A. bisporus (AB), and F. velutipes (FV), were used to evaluate and validate the LAMP-TP. Three hosts were detected positive by LAMP-TP (Figure S1). By contrast, all infected samples (No. 1 to 37) were detected positive by PCR using B3-Gr09 and F3-Gr09 primers (Figure S1). However, two samples (one from Chengdu and one from Jinan) were detected as positive by regular-PCR but negative by LAMP-TP.


Although a large number of the GR genes have been identified in insects, little is known about the olfactory system and mechanisms of Arachnida, which comprise over 100,000 named species, including spiders, scorpions, harvestmen, ticks, mites, and solifuges27. Our approach successfully identified low-expressing olfactory genes in a non-model mite species lacking genome sequences. We found that the GRs of three mites from the Acariformes were characterized into one subfamily, and low homology with the GRs from the Insecta. GRs are recognized as insect-specific chemosensory receptor families, expressed in gustatory receptor neurons (GRNs). Most GRs are classic seven transmembrane GPCRs involved in sweet and bitter taste reception and in the detection of non-volatile pheromones. However, there are four members of the GRs family that are expressed in ORNs, including two highly related GRs (GR21a and GR63a) that function in the detection of CO222,28. We did not identify these members of the GRs family in mites, but provided information for comparative and functional genomic analyses of 11 species from the Insecta and Arachnida.

We also developed a rapid detection assay for T. putrescentiae based on the GR gene and the Lamp method. There have been few reports on the application of the LAMP method for mite detection. We developed a color method for detecting T. putrescentiae in samples of fungi using test strips or SYBR Green I dispensed with gel electrophoresis. The sensitivity of LAMP-TP was 0.5 ng/μL and the assay duration was needed less than 60 min.

In summary, we established a LAMP-TP method specific for the detection of T. putrescentiae. This simple method has shorter detection time, high sensitivity, and strong specificity.



The T. putrescentiae strain studied originated from a population collected in 2012 on wood ear mushroom Auricularia polytricha in Feng County (Jiangsu, China). The mites were mass reared on P. ostreatus mycelia in the laboratory at 25 °C and 85% RH. The mites were cultured by methods reported previously9.

Transcriptome sequencing

Total RNAs were extracted using SV Total RNA Isolation System (Promega, Madison, WI, USA) from adults (about 300 males and females mixed) according to manufacturer protocol. The cDNA library construction and the Illumina HiSeq2000 sequencing were conducted at Novogene Company (Beijing, China). The abundances of the unigenes in the transcriptomes were calculated by the RPKM (Reads Per Kilobase per Million mapped reads) method, using the formula: RPKM (A) = (1,000,000 × C × 1,000)/(N × L), where RPKM (A) is the expression abundance of gene A; C is the number of reads that are uniquely mapped to gene A; N is the total number of reads that are uniquely mapped to all genes and L is the number of bases on gene A. The RPKM method is able to eliminate the influence of different gene lengths and sequencing discrepancies in the calculation of transcript abundance29.

Identification of chemoreceptor genes superfamily from the T. putrescentiae transcriptome

Transcriptome (without a reference genome) assembly was accomplished based on the left.fq and right.fq using Trinity with min_kmer_cov set to 2 by default and all other parameters set to default. Gene function was annotated based on the following databases: Nr (NCBI non-redundant protein sequences), Nt (NCBI non-redundant nucleotide sequences), Pfam (Protein family), KOG/COG (Clusters of Orthologous Groups of proteins), Swiss-Prot (A manually annotated and reviewed protein sequence database), KO (KEGG Ortholog database) and GO (Gene Ontology). Within these databases, GRs were identified by manually searching with the keywords “gustatory receptors”. The translated protein sequences of target genes were edited and subjected to BLAST online severs as well as further identification and analysis. TMHMM 2.0 ( was used to predict transmembrane domains of candidate GRs.

Sequence analysis and phylogenetic tree construction

GRs from T. putrescentiae identified in this study were aligned with the respective gene families from other arthropod species, D. melanogaster, A. gambiae, B. mori, A. aegypti, C. quinquefasciatus, I. scapularis, P. humanus, S. scabiei, T. urticae and M. occidentalis (Table S1). Genome sequence data and gene annotations were downloaded from public data repositories: D. melanogaster and B. mori from National Center for Biotechnology Information (, A. gambiae, A. aegypti, C. quinquefasciatus, P. humanus and I. scapularis from VectorBase (, M. occidentalis from Hoy et al. (2016)12. ORFs were identified and translated into amino acid sequences using Expasy software ( The putative N-terminal signal peptides of all predicted olfactory genes were predicted by SignalP 4.0 server version ( with more than 70 amino acids before conducting the analyses30. All sequence alignments were performed using ClustalX2.131. Phylogenetic trees were constructed by the neighbor-joining method with the Jones-Taylor-Thornton (JTT) amino acid substitution model as implemented in MEGA7.0 software and then edited in the Evolview server ( Bootstrap support of tree branches was assessed by resampling amino acid positions 1000 times.

Optimization of the LAMP detection system

DNA genome extraction

Six different total DNA samples were extracted from T. putrescentiae (TP), two other mushroom mites, R. robini and M. secunda, the fungus gnat, B. difformis, the mushroom pathogen, P. tolaasii, and from mycelia of the P. ostreatus host, using the Takara MiniBEST Viral DNA Extraction Kit Ver. 5.0 (Takara Biotechnology Co., Ltd., Dalian, China) according to the manufacturer instructions. The extracted DNAs were used as the templates in the LAMP assays.

LAMP procedure

We conducted a probe hybridization reaction experiment and determined the selected primers that exhibited no reaction during probe hybridization. Subsequently, the LAMP tests were conducted with different primer combinations based on the GR gene. The primers used in the LAMP assay to detect T. putrescentiae were designed in this study. The primers F3-Gr09, B3-Gr09, FIP-Gr09, and BIP-Gr09 (Table 1) were designed using online LAMP primer software PrimerExplorer ( The probes were labeled with FAM or biotin.

DNA genome extraction

LAMP reactions were performed in a total volume of 2 μL and contained 1.0 μL (10 pM) F3-Gr09 and B3-Gr09 primers, 4.0 μL (10 pM) the FIP and BIP primers, 9.5 μL (2.5 mM) of dNTPs, 2.5 μL of 10X Bst DNA polymerase buffer, 0.5 μL (8 U) of Bst DNA polymerase (New England BioLabs, Herts, UK), 2 μL of template DNA, 0.5 μL (100 mM) of MgSO 4. The amplifications were performed at 65 °C for 60 min and were terminated by incubating the reactions at 80 °C for 10 min. In addition to gel electrophoresis, both visual inspection and strip graph were used to detect positive reactions and validate the LAMP results. Upon addition of the SYBR green I dye to tubes after the LAMP reaction, the color changed to yellowish green in the positive reactions. The products of LAMP were dropped onto the sample pad of the test strips (Ustar Biotech, Hangzhou, China). The test strips were observed after 1 min. Positive LAMP-TP was denoted by two red lines, with the top line for quality control and the bottom line for the test. Only the control line is negative. Otherwise, only the test line is invalid.

Sensitivity assay

The sensitivity of the LAMP-TP assay was evaluated using template concentrations from 0.15 ng/μL to 50 ng/μL. The genome dilution series were used in the LAMP assay and in PCR to determine the minimum detection concentrations for each assay.

Optimization of LAMP-TP

To detect T. putrescentiae from clinical specimens, a LAMP assay system was optimized. LAMP assay optimization included concentrations, reaction temperature and reaction time. Reaction temperatures selected for the LAMP assays ranged from 58 °C to 65 °C. The reaction time was extended by 10 to 30 min, based on the optimum experimental conditions to determine the relationship between reaction time and sensitivity. The amplification results from the optimized LAMP assay were detected by gel electrophoresis, color changes, and strip graph.

LAMP-TP used for detection in clinical specimens

We collected 37 samples from four edible mushrooms, P. ostreatus, A. bisporus, A. polytricha, and F. velutipes, apparently infected with the storage mite from 3 regions (Beijing, Harbin, and Jinan) of China to evaluate the LAMP-TP method. Presence of mites in the samples was determined by microscopic examination. Total DNAs were extracted from the 37 samples according to manufacturer protocol.

We applied the PCR LAMP to detect T. putrescentiae in the samples to verify the clinical potential of the method. The same samples were tested using a PCR method with the detection primers F3-Gr09/B3-Gr09.


  1. 1.

    Erban, T. & Hubert, J. Digestive physiology of synanthropic mites (acari: Acaridida). SOAJ of Entomological Studies 1, 1–37 (2012).

    Google Scholar 

  2. 2.

    Zhang, G. & Jin, L. Species and distribution of stored product mites in china. Food Sci. Technol. Commun. 2, 23–24 (1960).

    Google Scholar 

  3. 3.

    Yong Jeong, K. et al. Molecular cloning and the allergenic characterization of tropomyosin from tyrophagus putrescentiae. Protein and Peptide Letters 14, 431–436 (2007).

    ADS  Article  Google Scholar 

  4. 4.

    Li, C. P., Cui, Y. B., Wang, J., Yang, Q. G. & Tian, Y. Acaroid mite, intestinal and urinary acariasis. World Journal of Gastroenterology: WJG 9, 874–877 (2003).

    Article  PubMed  Google Scholar 

  5. 5.

    Maraun, M. et al. Stable isotopes revisited: their use and limits for oribatid mite trophic ecology. Soil Biology and Biochemistry 43, 877–882 (2011).

    Article  CAS  Google Scholar 

  6. 6.

    Rohlfs, M. & Churchill, A. C. Fungal secondary metabolites as modulators of interactions with insects and other arthropods. Fungal Genetics and Biology 48, 23–34 (2011).

    Article  PubMed  CAS  Google Scholar 

  7. 7.

    Duek, L., Kaufman, G., Palevsky, E. & Berdicevsky, I. Mites in fungal cultures. Mycoses 44, 390–394 (2001).

    Article  PubMed  CAS  Google Scholar 

  8. 8.

    Kheradmand, K., Kamali, K., Fathipour, Y. & Goltapeh, E. M. Development, life table and thermal requirement of tyrophagus putrescentiae (astigmata: Acaridae) on mushrooms. Journal of Stored Products Research 43, 276–281 (2007).

    Article  Google Scholar 

  9. 9.

    Qu, S. X. et al. Temperature-dependent development and reproductive traits of tyrophagus putrescentiae (sarcoptiformes: Acaridae) reared on different edible mushrooms. Environmental Entomology 44, 392–399 (2015).

    Article  PubMed  CAS  Google Scholar 

  10. 10.

    Zhang, Y. X., Lin, J., Huang, J. & Zhu, P. Studies on tyrophagus putreseentiae (schrank) and its damage to the edible fungi. J. Fujian Agric. Sci 7, 91–94 (1992).

    Google Scholar 

  11. 11.

    Houck, M. A. Mites: ecological and evolutionary analyses of life-history patterns. Environmental Entomology 24, 1748–1749 (1993).

    ADS  Google Scholar 

  12. 12.

    Hoy, M. A. et al. Genome sequencing of the phytoseiid predatory mite metaseiulus occidentalis reveals completely atomized hox genes and superdynamic intron evolution. Genome Biology and Evolution 8, 1762–1775 (2016).

    Article  PubMed  PubMed Central  Google Scholar 

  13. 13.

    Asahina, K., Pavlenkovich, V. & Vosshall, L. B. The survival advantage of olfaction in a competitive environment. Current Biology 18, 1153–1155 (2008).

    Article  PubMed  CAS  Google Scholar 

  14. 14.

    De Bruyne, M. & Baker, T. Odor detection in insects: volatile codes. Journal of Chemical Ecology 34, 882–897 (2008).

    Article  PubMed  CAS  Google Scholar 

  15. 15.

    Leal, W. S. Odorant reception in insects: roles of receptors, binding proteins, and degrading enzymes. Annual review of entomology 58, 373–391 (2013).

    Article  PubMed  CAS  Google Scholar 

  16. 16.

    Stensmyr, M. C. et al. A conserved dedicated olfactory circuit for detecting harmful microbes in drosophila. Cell 151, 1345–1357 (2012).

    Article  PubMed  CAS  Google Scholar 

  17. 17.

    Niessen, L., Luo, J., Denschlag, C. & Vogel, R. F. The application of loop-mediated isothermal amplification (lamp) in food testing for bacterial pathogens and fungal contaminants. Food Microbiology 36, 191–206 (2013).

    Article  PubMed  CAS  Google Scholar 

  18. 18.

    Frkaczyk, M., Wozniakowski, G., Kowalczyk, A., Niemczuk, K. & Pejsak, Z. Development of cross-priming amplification for direct detection of the african swine fever virus, in pig and wild boar blood and sera samples. Letters in Applied Microbiology 62, 386–391 (2016).

    Article  CAS  Google Scholar 

  19. 19.

    Zeng, D. et al. Rapid diagnosis of soya bean root rot caused by fusarium culmorum using a loop-mediated isothermal amplification assay. Journal of Phytopathology 165, 249–256 (2017).

    ADS  Article  CAS  Google Scholar 

  20. 20.

    Lam, P., Keri, R. A. & Steinmetz, N. F. A bioengineered positive control for rapid detection of the ebola virus by reverse transcription loop-mediated isothermal amplification (rt-lamp). ACS Biomaterials Science & Engineering 3, 452–459 (2017).

    Article  CAS  Google Scholar 

  21. 21.

    Zhou, J. J. et al. Genome annotation and comparative analyses of the odorant-binding proteins and chemosensory proteins in the pea aphid acyrthosiphon pisum. Insect Molecular Biology 19, 113–122 (2010).

    ADS  Article  PubMed  CAS  Google Scholar 

  22. 22.

    Kwon, J. Y., Dahanukar, A., Weiss, L. A. & Carlson, J. R. The molecular basis of co2 reception in drosophila. Proceedings of the National Academy of Sciences 104, 3574–3578 (2007).

    ADS  Article  CAS  Google Scholar 

  23. 23.

    Wanner, K. & Robertson, H. The gustatory receptor family in the silkworm moth bombyx mori is characterized by a large expansion of a single lineage of putative bitter receptors. Insect Molecular Biology 17, 621–629 (2008).

    Article  PubMed  CAS  Google Scholar 

  24. 24.

    Kent, L. B., Walden, K. K. & Robertson, H. M. The gr family of candidate gustatory and olfactory receptors in the yellow-fever mosquito aedes aegypti. Chemical Senses 33, 79–93 (2007).

    Article  PubMed  CAS  Google Scholar 

  25. 25.

    Benton, R., Vannice, K. S., Gomez-Diaz, C. & Vosshall, L. B. Variant ionotropic glutamate receptors as chemosensory receptors in drosophila. Cell 136, 149–162 (2009).

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  26. 26.

    Yeh, H. Y., Shoemaker, C. A. & Klesius, P. H. Evaluation of a loop-mediated isothermal amplification method for rapid detection of channel catfish ictalurus punctatus important bacterial pathogen edwardsiella ictaluri. Journal of Microbiological Methods 63, 36–44 (2005).

    Article  PubMed  CAS  Google Scholar 

  27. 27.

    Cracraft, J. et al. Phylogenetic relationships among modern birds (neornithes). 468–489 (Oxford University Press New York, Oxford, 2004).

  28. 28.

    Scott, K. et al. A chemosensory gene family encoding candidate gustatory and olfactory receptors in drosophila. Cell 104, 661–673 (2001).

    Article  PubMed  CAS  Google Scholar 

  29. 29.

    Grabherr, M. G. et al. Full-length transcriptome assembly from rna-seq data without a reference genome. Nature Biotechnology 29, 644–652 (2011).

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  30. 30.

    Petersen, T. N., Brunak, S., von Heijne, G. & Nielsen, H. Signalp 4.0: discriminating signal peptides from transmembrane regions. Nature Methods 8, 785–786 (2011).

    Article  PubMed  CAS  Google Scholar 

  31. 31.

    Thompson, J. D., Gibson, T. J., Plewniak, F., Jeanmougin, F. & Higgins, D. G. The clustal_x windows interface: flexible strategies for multiple sequence alignment aided by quality analysis tools. Nucleic Acids Research 25, 4876–4882 (1997).

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  32. 32.

    He, Z. L. et al. Evolview v2: an online visualization and management tool for customized and annotated phylogenetic trees. Nucleic Acids Research 44, W236–W241 (2016).

    Article  PubMed  PubMed Central  CAS  Google Scholar 

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We are grateful for the financial support provided by Modern Agro-industry Technology Research System of China (No: CARS-20) and the Natural Science Foundation of Jiangsu Province (No. BK20170612). We thank LetPub ( for providing linguistic assistance during manuscript preparation.

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S.-X.Q. designed the experiments. S.-X.Q., X.-F.W. and H.-P.L. wrote the main manuscript. X.-F.W. carried out bioinformatics analysis. H.-P.L. performed the statistical analyses and figures. X.L. performed the PCR experiments. S.-X.Q., H.-P.L. and L.M. analyzed the data. S.-X.Q. and H.-P.L. revised the manuscript.

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Correspondence to Shao-Xuan Qu.

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Qu, SX., Wang, XF., Li, HP. et al. A Gustatory Receptor Used for Rapid Detection of Tyrophagus putrescentiae in Fungi Hosts. Sci Rep 8, 11425 (2018).

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