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- M. Mohan
- K. Subaharan
- T. Venkatesan
- Sanjay Yelshetti
- M. Kannan
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- M. S. Yandigeri
- Surabhi Kumari
- K. Elango
- P. Ram Kumar
- R. Rangeshwaran
- Mahesh S. Yandigeri
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Sivakumar, G.
- Gut bacteria mediated insecticide resistance in cotton leafhopper Amrasca biguttula biguttula
Abstract Views :208 |
PDF Views:93
Authors
G. Sivakumar
1,
M. Mohan
1,
K. Subaharan
1,
T. Venkatesan
1,
Sanjay Yelshetti
1,
M. Kannan
2,
R. Anandham
3,
M. S. Yandigeri
1,
Surabhi Kumari
1,
K. Elango
4,
P. Ram Kumar
1
Affiliations
1 ICAR-National Bureau of Agricultural Insect Resources, Bengaluru 560 024, IN
2 Department of Nanoscience and Technology, Tamil Nadu Agricultural University, Coimbatore 641 003, IN
3 Department of Agricultural Microbiology, Tamil Nadu Agricultural University, Coimbatore 641 003, IN
4 Department of Agricultural Entomology, Kumaraguru Institute of Agriculture, Erode 638 315, IN
1 ICAR-National Bureau of Agricultural Insect Resources, Bengaluru 560 024, IN
2 Department of Nanoscience and Technology, Tamil Nadu Agricultural University, Coimbatore 641 003, IN
3 Department of Agricultural Microbiology, Tamil Nadu Agricultural University, Coimbatore 641 003, IN
4 Department of Agricultural Entomology, Kumaraguru Institute of Agriculture, Erode 638 315, IN
Source
Current Science, Vol 122, No 8 (2022), Pagination: 958-964Abstract
Cotton leafhopper, Amrasca biguttula biguttula (Ishida) (Hemiptera: Cicadellidae) is a major sucking insect pest of cotton in India. Indiscriminate use of pesticides has led to the development of resistance to most of the recommended pesticide groups. Though there are multiple mechanisms and principles of insecticide resistance development in insects, the gut bacterial-mediated degradation of insecticides is relatively less explored. In the present study, the gut bacteria of field-collected, insecticide-resistant population of A. biguttula biguttula were compared with a laboratory-reared susceptible population. Among the five culturable gut bacteria from the imidacloprid-resistant population, only Enterococcus silesiacus CLHG1a exhibited growth in the agar medium amended with 50 and 100 ppm of imidacloprid. The imidacloprid degrading capacity of E. silesiacus CLHG1a was further confirmed by HPLC analysis. E. silesiacus and Bacillus amyloliquefaciens CLHG2 showed higher esterolytic activity (0.348 and 0.309 mmoles/min/mg respectively). The esterase zymogram on native PAGE revealed a single major band. This study provides clear evidence that the bacterium E. silesiacus isolated from the gut of A. biguttula biguttula has the ability to degrade imidacloprid and may have played a role in the detoxification of pesticides.Keywords
Cotton, detoxification, esterase activity, gut microflora, insecticide resistance, leafhopper.References
- Anon., All India Coordinated Cotton Improvement Project. Central Institute for Cotton Research, Coimbatore, 2009, pp. 9–15.
- Mohan, M. and Katiyar, K. N., Impact of different insecticides used for bollworm control on the population of jassid and whitefly in cotton. Pestic. Res. J., 2000, 12, 99–102.
- Kannan, M., Uthamasamy, S. and Mohan, S., Impact of insecticides on sucking pests and natural enemy complex of transgenic cotton. Curr. Sci., 2004, 86, 726–729.
- Jeya, P. S. and Regupathy, A., Generating base line data for insecticide resistance monitoring in cotton leafhopper, Amrasca devastans (Distant). Resist. Pest Manage. Newsl., 2002, 11, 4–5.
- Koga, R. and Moran, N. A., Swapping symbionts in spittlebugs: evolutionary replacement of a reduced genome symbiont. ISME J., 2014, 8, 1237–1246.
- Kranthi, K. R., Insecticide resistance management in cotton to enhance productivity. Model training course on cultivation of long staple cotton (ELS), Central Institute for Cotton Research, Regional Station, Coimbatore, 2007, pp. 214–231.
- Kranthi, S., Kranthi, K. R., Rodge, C., Chawla, S. and Nehare, S., Insect resistance to insecticides and Bt cotton in India. In Natural Resource Management: Ecological Perspectives (eds Peshin, R. and Dhawan, A. K.), Springer Nature, Switzerland, 2020, pp. 185– 199.
- Saeed, R., Muhammad, R., Naeem, A., Muhammad, T. J. and Muhammad, N., Toxicity and resistance of the cotton leafhopper Amrasca devastans (Distant) to neonicotinoid insecticides in Punjab, Pakistan. Crop Prot., 2017, 93, 143–147.
- Kikuchi, Y., Hosokawa, T. and Fukatsu, T., An ancient but promiscuous host–symbiont association between Burkholderia gut symbionts and their heteropteran hosts. ISME J., 2011, 5, 446–460.
- Douglas, A. E., The microbial dimension in insect nutritional ecology. Funct. Ecol., 2009, 23, 38–47.
- Sivakumar, G. et al., Characterization and role of gut bacterium Bacillus pumilus on nutrition and defense of leafhopper Amrasca biguttula biguttula (Ishida) of cotton in India. Indian J. Agric. Sci., 2017, 87, 534–539.
- Broderick, N. A., Raffa, K. F. and Handelsman, J., Midgut bacteria required for Bacillus thuringiensis insecticidal activity. Proc. Natl. Acad. Sci. USA, 2006, 103(41), 15196–15199.
- Cariveau, D. P., Powell, J. E., Koch, H., Winfree, R. and Moran, N. A., Variation in gut microbial communities and its association with pathogen infection in wild bumblebees (Bombus). ISME J., 2014, 8, 2369–2379.
- Jaenike, J., Unckless, R., Cockburn, S. N., Boelio, L. M. and Perlman, S. J., Adaptation via symbiosis: recent spread of a drosophila defensive symbiont. Science, 2010, 329, 212–215.
- Sharon, G., Segal, D., Ringo, J. M., Hefetz, A., Zilber-Rosenberg, I. and Rosenberg, E., Commensal bacteria play a role in mating preference of Drosophila melanogaster. Proc. Natl. Acad. Sci. USA, 2010, 107, 20051–20056.
- Montllor, C. B., Maxmen, A. and Purcell, A. H., Facultative bacterial endosymbionts benefit pea aphids Acyrthosiphon pisum under heat stress. Ecol. Entomol., 2002, 27, 189–195.
- Desai, M. S. and Brune, A., Bacteroidales ectosymbionts of gut flagellates shape the nitrogen-fixing community in dry-wood termites. ISME J., 2012, 6, 1302–1313.
- Senderovich, Y. and Halpern, M., The protective role of endogenous bacterial communities in chironomid egg masses and larvae. ISME J., 2013, 7, 2147–2158.
- Ben-Yosef, M., Pasternak, Z., Jurkevitch, E. and Yuval, B., Symbiotic bacteria enable olive fly larvae to overcome host defences. R. Soc. Open Sci., 2015, 2, 150–170.
- Cejanavarro, J. A. et al., Gut microbiota mediate caffeine detoxification in the primary insect pest of coffee. Nature Commun., 2015, 6, 7618.
- Kikuchi, Y., Hayatsu, M., Hosokawa, T., Nagayama, A., Tago, K. and Fukatsu, T., Symbiont-mediated insecticide resistance. Proc. Natl. Acad. Sci. USA, 2012, 109, 8618–8622.
- Sivakumar, G., Rangeshwaran, R., Yandigeri, M. S., Mohan, M., Venkatesan, T. and Vergheses, A., Diversity of culturable gut bacteria associated with the field populations of cotton leafhopper Amrasca biguttula biguttula (Ishida) in India. Indian J. Agric. Sci., 2016, 86, 208–215.
- Xia, X., Sun, B., Gurr, G. M., Vasseur, L., Xue, M. and You, M., Gut microbiota mediate insecticide resistance in the diamondback moth, Plutella xylostella (L.). Front Microbiol., 2018, 9, 25.
- Fusetto, R., Shane, D., Trent, P., Richard, A. J., Hair, O. and Philip, B., Partitioning the roles of CYP6G1 and gut microbes in the metabolism of the insecticide imidacloprid in Drosophila melanogaster. Sci. Rep., 2017, 7, 1–12.
- Ramya, S. L., Venkatesan, T., Srinivasa, M. K., Jalali, S. K. and Abraham, V., Detection of carboxylesterase and esterase activity in culturable gut bacterial flora isolated from diamondback moth,
- Plutella xylostella (Linnaeus), from India and its possible role in indoxacarb degradation. Braz. J. Microbiol., 2016, 47, 327–336.
- Indiragandhi, P., Yoon, Ch., Oh Yang, J., Cho, S., Sa, T. M. and Kim, G. H., Microbial communities in the developmental stages of B and Q biotypes of sweet potato whitefly, Bemisia tabaci (Hemiptera: Aleyrodidae). J. Korean Soc. Appl. Biol. Chem., 2010, 53(5), 605–617.
- Saranya, M., Kennedy, J. S., Jeyarani, S. and Anandham, R., Parasitic potential of Encarsia guadeloupae Viggiani (Hymenoptera: Aphelinidae) on Aleurodicus rugioperculatus Martin (Hemiptera:
- Aleyrodidae). Phytoparasitica, 2021, p. 141.
- Heong, K. L., Tan, K. H., Garcia, C. P. F., Liu, Z. and Lu, Z., Research Methods in Toxicology and Insecticide Resistance Monitoring of Rice Planthoppers, International Rice Research Institute, Los Baños, Philippines, 2013, 2nd edn.
- Feng, W., Wang, X. Q., Zhou, W., Liu, G. Y. and Wan, Y. J., Isolation and characterization of lipase producing bacteria in the intestine of the silkworm, Bombyx mori, reared on different forage. J. Insect Sci., 2011, 11, 135.
- Harley, J. P. and Prescott, L. M., In Laboratory Exercises in Microbiology, The McGraw-Hill Companies, New York, USA, 2002.
- Meghji, K., Ward, O. P. and Araujo, A., Production, purification, and properties of extracellular carboxyl esterases from Bacillus subtilis NRRL 365. Appl. Environ. Microbiol., 1990, 56, 3735–3740.
- Chandrashekharaiah, K. S., Swamy, N. R. and Murthy, K. R., Carboxylesterases from the seeds of an underutilized legume, Mucuna pruriens: isolation, purification and characterization. Phytochemistry, 2011, 72, 2267–2277.
- Hunter, R. L. and Markert, L., Histochemical demonstration of enzymes separated by zone electrophoresis in starch gels. Science, 1957, 125, 1294–1295.
- Honnappagouda, K., Bheemanna, M. and Suhas, Y., Current efficacy status of imidacloprid formulations against okra leafhopper, Amrasca biguttula biguttula. Indian J. Plant Prot., 2011, 39, 70–72.
- Dunbar, H. E., Wilson, A. C., Ferguson, N. R. and Moran, N. A., Aphid thermal tolerance is governed by a point mutation in bacterial symbionts. PLoS Biol., 2007, 5, 1006–1015.
- Snehaa, C. P., Hemalatha, B. N., Reetha, B., Venkatesan, T. and Jalali, S. K., Molecular characterization of microbes associated with cotton mealy bug, Phenacoccus solenopsi Tinsley. In New Horizons in Insect Science, International Conference on Insect Science, Bengaluru, 2013, pp. 14–17.
- Caspi-Fluger, A., Inbar, M., Mozes-Daube, N., Mouton, L., Hunter, M. S. and Zchori-Fein, E., Rickettsia ‘in’ and ‘out’: two different localization patterns of a bacterial symbiont in the same insect species. PLoS ONE, 2011, 6(6), 21096.
- Werren, J. H. and O’Neill, S. L., The evolution of heritable symbionts. In Influential Passengers: Inherited Microorganisms and Arthropod Reproduction, Oxford University Press, Oxford, 1997, pp. 1–41.
- Shao, Y., Arias-Cordero, E., Guo, H., Bartram, S. and Boland, W., In vivo Pyro-SIP assessing active gut microbiota of the cotton leafworm, Spodoptera littoralis. PLoS ONE, 2014, 9, 85948.
- Xiang, H. et al., Microbial communities in the larval midgut of laboratory and field populations of cotton bollworm (Helicoverpa armigera). Can. J. Microbiol., 2006, 52, 1085–1092.
- Lauzon, C. R., Potter, S. and Prokopy, R. J., Degradation and detoxification of the dihydrochalcone phloridzin by Enterobacter agglomerans, a bacterium associated with the apple pest, Rhagoletis pomonella (Walsh) (Diptera: Tephritidae). Environ. Entomol., 2003, 32, 953–963.
- Pandey, G., Dorrian, S. J., Russell, R. J. and Oakeshott, J. G., Biotransformation of the neonicotinoid insecticides imidacloprid and thiamethoxam by Pseudomonas sp. 1G. Biochem. Biophys. Res. Commun., 2009, 380, 710–714.
- Yalashetti, S., Yandigeri, M. S., Rudrappa, O., Mohan, M. and Sivakumar, G., Diversity of culturable and unculturable gut bacteria associated with field population of Spodoptera litura (Fab). Bull. Environ. Pharmacol. Life Sci., 2017, 6, 441–451.
- Cheng, D., Guo, Z., Riegler, M., Xi, Z., Liang, G. and Xu, Y., Gut symbiont enhances insecticide resistance in a significant pest, the oriental fruit fly Bactrocera dorsalis (Hendel). Microbiome, 2017, 5, 13.
- Anhalt, J. C., Moorman, T. B. and Koskinen, W. C., Biodegradation of imidacloprid by an isolated soil microorganism. J. Environ. Sci. Health, 2007, 42, 509–514.
- Natural Occurrence of Entomopathogens on the Invasive Fall Armyworm, Spodoptera Frugiperda (j.e. Smith) in South India
Abstract Views :253 |
PDF Views:90
Authors
G. Sivakumar
1,
M. Mohan
1,
M. Kannan
2,
K. Elango
3,
P. Ram Kumar
1,
T. Venkatesan
1,
R. Rangeshwaran
1,
Mahesh S. Yandigeri
1,
O. Dhanyakumar
1
Affiliations
1 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, IN
2 Department of Nanoscience and Technology, Periyakulam, Tamil Nadu Agricultural University, Coimbatore 641 003, IN
3 Horticultural Research Station, Tamil Nadu Agricultural University, Kodaikanal 624 103, IN
1 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, IN
2 Department of Nanoscience and Technology, Periyakulam, Tamil Nadu Agricultural University, Coimbatore 641 003, IN
3 Horticultural Research Station, Tamil Nadu Agricultural University, Kodaikanal 624 103, IN
Source
Current Science, Vol 120, No 4 (2021), Pagination: 619-621Abstract
No Abstract.References
- Sharanabasappa, D. et al., Pest Manage. Hort. Ecosyst., 2018, 24, 23–29.
- Shylesha, A. N. et al., J. Biol. Control, 2018, 32(3), 145–151.
- Mallapur, C. P., Naik, A. K., Hagari, S. Praveen, T., Patil, R. K. and Lingappa, S., J. Entomol. Zool. Stud., 2018, 6(6), 1062–1067.
- Raghunandan, B. L., Patel, N. M., Dave, H. J. and Mehta, D. M., J. Entomol. Zool. Stud., 2019, 7(2), 1040–1043.
- Sharanabasappa, D., Kalleshwaraswamy, C. M., Poorani, J., Maruthi, M. S., Pavithra, H. B. and Diraviam, J., Fla. Entomol., 2019, 1029(2), 619–623.
- Firake, D. M. and Behere, G. T., Biol. Control, 2020, 148, 104303.
- Sivakumar, G. et al., Curr. Sci., 2020, 119, 5.
- Vellend, M., J. Veg. Sci., 2001, 12, 545– 552.
- Sun, B. D. and Liu, X. Z., Appl. Soil Ecol., 2008, 39(1), 100–108.
- Okrikata, E. and Yusuf, O. A., Int. Biol. Biomed. J. Autumn, 2016, 2, 4.
- Suby, S. B. et al., Curr. Sci., 2020, 119(1), 44–51.
- Prasanna, B. M., Huesing, J. E., Eddy, R. and Peschke, V. M., Fall armyworm in Africa: a guide for integrated pest management, CIMMTY, Mexico, 2018, p.109.
- Sinha, K. K., Choudhary, A. K. and Priyanka Kumari, Entomopathogenic fungi, In Ecofriendly Pest Management for Food Security (ed. Omkar), Elsevier, Academic Press, Cambridge, USA, 2016, pp. 475–505.
- Monnerat, R. G. and Bravo, A., Controle Biol., 2000, 3, 163–200.
- Kepler, R. M., Humber, R. A., Bischoff, J. F. and Rehner, S. A., Mycologia, 2014, 106(4), 811–829.
- Enhanced Insecticide-resistance Spectrum in Green Lacewing Predator, Chrysoperla zastrowi sillemi (strain PTS-8) And Its Potential Role In The Management Of Sucking Pests Of Cotton
Abstract Views :247 |
PDF Views:90
Authors
Affiliations
1 Department of Entomology, University of Agricultural Sciences, Gandhi Krishi Vignan Kendra, Bellary Road, Bengaluru 560 065, IN
2 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, IN
1 Department of Entomology, University of Agricultural Sciences, Gandhi Krishi Vignan Kendra, Bellary Road, Bengaluru 560 065, IN
2 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, IN
Source
Current Science, Vol 120, No 2 (2021), Pagination: 423-428Abstract
The green lacewing or aphid lion, Chrysoperla zastrowi sillemi (Esben-Petersen) is an important predator of sucking pests, and eggs and neonate larvae of lepiodopteran pests under many crop ecosystems of India. In the present study, enhanced insecticide resistance spectrum in an insecticide-resistant population of C. zastrowi sillemi (strain PTS-8) was evaluated against four commonly used insecticides on cotton. The insecticide resistant C. zastrowi sillemi PTS-8 showed 16.4-, 14.8-, 12.7- and 7.2-fold resistance against chlorpyriphos 20% EC, cypermethrin 10% EC, acetamipirid 20% SP and chlorantraniliprole 18.5% SC respectively, compared to the susceptible strain. Biochemical assays revealed an elevated level of three major detoxifying enzymes, viz. carboxylesterase (1.48-fold), glutathione S-transferase (1.27-fold) and cytochrome p450 monooxygenase (1.36-fold) in PTS-8 strain compared to the susceptible strain. The field survival and biocontrol potential of PTS-8 strain were significantly better on cotton plants treated with recommended dose of insecticides. The study indicated the potential role of insecticide-resistant natural enemies under biointensive IPM programmes to avoid compatibility conflict with insecticides.Keywords
Chrysoperla zastrowi sillemi, Cotton, Detoxifying Enzymes, Insecticide Resistance, Sucking Pests.References
- Dhandapani, N., Pallavi, S. and Mishra, G., Chrysopids. In Ecofriendly Pest Management for Food Security (ed. Omkar), Elsevier, San Diego, USA, 2016, pp. 311–327.
- Henry, C. S., Brooks, S. J., Johnson, J. B., Venkatesan, T. and Duelli, P., The most important lacewing species in Indian agricultural crops, Chrysoperla sillemi (Esben-Petersen), is a subspecies of Chrysoperla zastrowi (Esben-Petersen) (Neuroptera: Chrysopidae). J. Nat. Hist., 2010, 44, 2543–2555; https://doi.org/ 10.1080/00222933.2010.499577.
- Pappas, M. L., Broufas, G. D. and Koveos, D. S., Chrysopid predators and their role in biological control. J. Entomol., 2011, 8(3), 301–326; https://doi.org/10.3923/je.2011.301.326.
- Senior, L. J. and McEwen, P. K., The use of lacewings in biological control. In Lacewings in the Crop Environment (eds McEwen, P. K., New, T. R. and Whittington, A. E.), Cambridge University Press, Cambridge, UK, 2011, pp. 296–299.
- Venkatesan, T., Mahiba, S. H., Jalali, S., Ramya, S. and Pratibha, M., Detection of insecticide resistance and mechanisms of resistance in field populations of Chrysoperla zastrowi sillemi (Neuroptera: Chrysopidae) collected from different geographical locations in India. J. Biol. Control, 2017, 31(3), 61–68; https:// doi.org/10.18311/jbc/2017/16333.
- Roush, R. T. and Daly. J. C., The role of population genetics in resistance research and management. In Pesticide Resistance in Arthropods (eds Roush, R. T. and Tabashnik B. E.), Springer, USA, 1990, pp. 97–152.
- Pree, D. J., Archibald, D. E. and Morrison, R. K., Resistance to insecticides in the common green lacewing Chrysoperla carnea (Neuroptera: Chrysopidae) in southern Ontario. J. Econ. Entomol., 1989, 82(1), 29–34; https://doi.org/10.1093/jee/82.1.29.
- Daane, K. M., Ecological studies of released lacewings in crops. In Lacewings in the Crop Environment (eds McEwen, P. K., New, T. R. and Whittington, A. E.), Cambridge University Press, Cambridge, UK, 2001, pp. 338–345.
- Mansoor, M. M. and Shad, S. A., Genetics, cross-resistance and realized heritability of resistance to acetamiprid in generalist predator, Chrysoperla carnea (Steph.) (Neuroptera: Chrysopidae). Egypt. J. Biol. Pest Control, 2020, 30, 23; https://doi.org/10.1186/ s41938-020-0213-x.
- Easterbrooka, M. A., Fitzgeralda, J. D. and Solomona, M. G., Suppression of aphids on strawberry by augmentative releases of larvae of the lacewing Chrysoperla carnea (Stephens), Biocontrol Sci. Technol., 2006, 16(9), 893–900; https://doi.org/10.1080/ 09583150600827850.
- Venkatesan, T., Singh, S. P. and Jalali, S. K., Rearing of Chrysoperla carnea (Neuroptera: Chrysopidae) on semi-synthetic diet and its predatory efficiency against cotton pests. Entomon, 2000, 25(2), 81–89.
- Venkatesan, T., Singh, S. P., Jalali, S. K. and Joshi, S., Evaluation of predatory efficiency of Chrysoperla carnea (Stephens) reared on artificial diet against tobacco aphid Myzus persicae (Sultzer) in comparison with other predators. J. Entomol. Res., 2002, 26(3), 193–196.
- Panini, M., Manicardi, G. C., Moores, G. D. and Mazzoni, E., An overview of the main pathways of metabolic resistance in insects. Invertebr. Surviv. J., 2016, 13(1), 326–335; https://doi.org/ 10.25431/1824-307X/isj.v13i1.326-335.
- Oakeshott, J. G., Claudianos, C., Campbell, P. M., Newcomb, R. D. and Russell, J. R., Biochemical genetics and genomics of insect esterases. In Comprehensive Molecular Insect Science (eds Gilbert, L. I., Iatro, K. and Gill, S.), Elsevier, The Netherlands, 2010, pp. 1–73.
- Pathan, A. K., Sayyed, A. H., Aslam, M., Razaq, M., Jilani, G. and Saleem, M. A. Evidence of field-evolved resistance to organophosphates and pyrethroids in Chrysoperla carnea (Neuroptera: Chrysopidae). J. Econ. Entomol., 2008, 101(5), 1676–1684; https://doi.org/10.1093/jee/101.5.1676.
- Bradford, M. M., A rapid and sensitive method for the quantification of microgram quantities of protein utilizing the principle of protein-dye binding. Anal. Biochem., 1976, 74, 248–254; https://doi.org/10.1016/0003-2697(76)90527-3.
- Van Asperen, K., A study of housefly esterases by means of a sensitive colorimetric method. J. Insect Physiol., 1962, 8, 401–416; https://doi.org/10.1016/0022-1910(62)90074-4.
- Davis, B. J., Disc electrophoresis II. Method and application to human serum proteins. Ann. NY Acad. Sci., 1964, 121, 404–427; https://doi.org/10.1111/j.1749-6632.1964.tb14213.x.
- Kao, C. H., Hung, C. F. and Sun, C. N., Parathion and methyl parathion resistance in diamondback moth (Lepidoptera: Plutellidae) larvae. J. Econ. Entomol., 1989, 82(5), 1299–1304; https:// doi.org/10.1093/jee/82.5.1299.
- Kinoshita, F. K., Frawley, J. P. and Du Bois, K. P., Quantitative measurement of induction of hepatic microsomal enzymes by various dietary levels of DDT and toxaphene in rats. Toxicol. Appl. Pharmacol., 1966, 9, 505–511; https://doi.org/10.1016/0041008X(66)90011-1.
- Abbott, W. S., A method of computing the effectiveness of an insecticide. J. Econ. Entomol., 1925, 18(2), 265–267; https://doi.org/ 10.1093/jee/18.2.265a.
- Finney, D. J., Probit Analysis: A Statistical Treatment of the Sigmoid Response Curve, Cambridge University Press, Cambridge, UK, 1952, p. 318.
- Kim, Y. J., Lee, H. S., Lee, S. W., Kim, G. H. and Ahn, Y. J., Toxicity of tebufenpyrad to Tetranychus urticae (Acari: Tetranychidae) and Amblyseius womersleyi (Acari: Phytoseiidae) under laboratory and field conditions. J. Econ. Entomol., 1999, 92(1), 187–192; https://doi.org/10.1093/jee/92.1.187.
- Sohail, M., Nasar, M. H., Muhammad, R., Soomro, Q. A., Asif, M. U. and Maari, J. M., Resistance potential of Chrysoperla carnea (Stephens) to insecticides used against sucking complex of cotton. Int. J. Ecotoxicol. Ecobiol., 2019, 4(1), 1–7; https:// doi.org/10.11648/J.IJEE.20190401.11.
- Ishaaya, I., Insect detoxifying enzymes: their importance in pesticide synergism and resistance. Arch. Insect Biochem. Physiol., 1993, 22(1–2), 263–276; https://doi.org/10.1002/arch.940220119.
- Mohan, M. and Gujar, G. T., Local variation in susceptibility of the diamondback moth, Plutella xylostella (Linnaeus) to insecticides and role of detoxification enzymes. Crop Prot., 2003, 22(3), 495–504; https://doi.org/10.1016/S0261-2194(02)00201-6.
- Grafton-Cardwell, E. E. and Hoy, M. A., Genetic improvement of common green lacewing, Chrysoperla carnea (Neuroptera: Chrysopidae): selection for carbaryl resistance. Environ. Entomol., 1986, 15(6), 1130–1136; https://doi.org/10.1093/ee/15.6.1130.
- Mehrab, C., Mohammad, S. A., Breza, M. S., Browshan, A. B. and Banwara, B., Esterase banding pattern in different developmental stages of Culex quinquefasciatus Say 1823 (Diptera: Culicidae). Int. J. Adv. Biol. Res., 2016, 6(4), 553–557.
- Wu, Y., Detection and mechanisms of resistance evolved in insects to Cry toxins from Bacillus thuringiensis. Adv. Insect Physiol., 2014, 47, 297–342; https://doi.org/10.1016/B978-0-12800197-4.00006-3.
- Luo, C., Jones, C., Devine, G., Zhang, F., Denholm, I. and Gorman, K., Insecticide resistance in Bemisia tabaci biotype Q (Hemiptera: Aleyrodidae) from China. Crop Protect., 2010, 29, 429–434; https://doi.org/10.1016/j.cropro.2009.10.001.
- Characterization of granulosis viruses of sugarcane early shoot borer, Chilo infuscatellus (Snell.) and internode borer, Chilo sacchariphagus indicus (Kapur)
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Authors
Affiliations
1 Nano Science and Technology, Tamil Nadu Agricultural University, Coimbatore 641 003, IN
2 ICAR-Sugarcane Breeding Institute, Coimbatore 641 007, IN
3 Imayam Institute of Agriculture and Technology, Tiruchirappalli 621 206, IN
4 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, IN
1 Nano Science and Technology, Tamil Nadu Agricultural University, Coimbatore 641 003, IN
2 ICAR-Sugarcane Breeding Institute, Coimbatore 641 007, IN
3 Imayam Institute of Agriculture and Technology, Tiruchirappalli 621 206, IN
4 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, IN
Source
Current Science, Vol 121, No 4 (2021), Pagination: 570-573Abstract
A study was undertaken to characterize the granulosis viruses (GVs) of early shoot borer, Chilo infuscatellus (Snell.) (Crambidae: Lepidoptera) and internode borer, Chilo sacchariphagus indicus (Kapur) (Lepidoptera: Crambidae) in sugarcane. Scanning electron photomicrographs revealed ovo-cylindrical occlusion bodies (OBs) of GVs in early shoot and internode borers with an average size of 425.03 and 230.21 nm, 387.64 and 208.68 nm in length and breadth respectively. Transmission electron photomicrographs also showed ovo-cylindrical OBs embedded with a rod-shaped virion. The average length and breadth of the virion in the OB was 271.0 ´ 52.6 nm, 257.0 ´ 50.2 nm for early shoot and internode borer GVs respectively. Toxicity studies with the respective GVs revealed lethal concentration values of 4.38, 4.61, 6.89 OBs/mm2 and 1.85, 135.43, 8045.27 OBs/mm2 to second, third and fourth larval instars of Chilo infuscatellus granulosis virus (ChinGV) and Chilo sacchariphagus indicus granulosis virus (ChsaGV) respectively.Keywords
Early shoot borer, granulosis viruses, internode borer, occlusion bodies, sugarcane, toxicity.References
- Srikanth, J., Salin, K. P. and Jayanti, R., Sugarcane pests and their management. Sugarcane Breeding Institute (ICAR), Coimbatore, 2012, p. 91.
- Shyamrao, I. D. and Kumar, A., Sugarcane borers: a major threat to sugarcane production in India and their management. Biotica Res. Today, 2020, 2, 225–228.
- Moscardi, F., Assessment of the application of baculoviruses for control of Lepidoptera. Annu. Rev. Entomol., 1999, 44, 257–289.
- Melamed-Madjar, V. and Raccah, B., The trans-stadial and vertical transmission of a granulosis virus from the corn borer, Sesamia nonagroides. J. Invertebr. Pathol., 1979, 33, 259–264.
- Easwaramoorthy, S. and Santhalakshmi, G., Efficacy of granulosis virus in the control of shoot borer, Chilo infuscatellus Snellen. J. Biol. Control, 1988, 2, 26–28.
- Rao, N. V. and Babu, T. R., Field efficacy of granulosis virus for the control of sugarcane early shoot borer, Chilo infuscatellus Snellen. J. Biol. Control, 2005, 19, 145–148.
- Subramanian, S., Rabindra, R. J. and Sithanantham, S., Genetic and biological variations among Plutella xylostella granulovirus isolates. Phytoparasitica, 2008, 36, 220–230.
- Sivakumar, G. et al., Isolation and characterization of indigenous nucleopolyhedrovirus infecting new invasive Fall armyworm Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae) in India. Curr. Sci., 2020, 119, 860–864.
- Polo-PC, User’s guide to probit or logit analysis. LeOra Software, Berkeley, 1994.
- Kathleen, A., Tweeten, L. A., Bulla, J. R. and Richard, A. C., Isolation and purification of a granulosis virus from infected larvae of the Indian Meal Moth, Plodia interpunctella. Appl. Environ. Microbiol., 1977, 34, 320–327.
- Sciocco-Cap, A., Parola, A. D., Goldberg, A. V., Ghiringhelli, P. D. and Romanowski, V., Characterization of a granulovirus isolated from Epinotia aporema Wals. (Lepidoptera: Tortricidae) larvae. Appl. Environ. Microbiol., 2001, 67, 3702–3706.
- Naveen Kumar, P., Prasad, Y. G., Prabhakar, M., Phanidhara, A. and Venkateshwarlu, B., Granulovirus of semilooper, Achaea janata L. (Lepidoptera: Noctuidae): its bioefficacy and safety in mammalian toxicity tests. J. Biol. Control, 2013, 27, 99–104.
- Cuartas, P., Barrera, G., Barreto, E. and Villamizar, L., Characterization of a Colombian granulovirus (Baculoviridae: Betabaculovirus) isolated from Spodoptera frugiperda (Lepidoptera: Noctuidae) larvae. Bio. Sci. Tech., 2014, 24, 1265–1285.
- Ardisson-Araújo, D. M. et al., Betabaculovirus encoding a gp64 homolog. BMC Genomics, 2016, 17; https://doi.org/10.1186/s12864-016-2408-9.
- Isolation and Characterization of Indigenous Nucleopolyhedrovirus Infecting Fall Armyworm, Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae) in India
Abstract Views :242 |
PDF Views:86
Authors
G. Sivakumar
1,
M. Kannan
2,
S. Ramesh Babu
3,
M. Mohan
1,
M. Sampath Kumar
1,
P. Raveendran
1,
T. Venkatesan
1,
R. Rangeshwaran
1,
Chandish R. Ballal
1,
P. Ram Kumar
1
Affiliations
1 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, IN
2 Department of Plant Protection, Horticultural College and Research Institute, Periyakulam, Tamil Nadu Agricultural University, Coimbatore 641 003, IN
3 Agricultural Research Station, Borwat Farm, MPUAT, Banswara 327 001, IN
1 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, IN
2 Department of Plant Protection, Horticultural College and Research Institute, Periyakulam, Tamil Nadu Agricultural University, Coimbatore 641 003, IN
3 Agricultural Research Station, Borwat Farm, MPUAT, Banswara 327 001, IN
Source
Current Science, Vol 119, No 5 (2020), Pagination: 860-864Abstract
Fall armyworm (FAW), Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae) is an invasive insect pest of maize in India. Natural occurrence of nucleopolyhedrovirus (NPV) infection on S. frugiperda larvae was recorded in 2018 during surveys conducted in maize fields in Chikkaballapura district of Karnataka, and Coimbatore and Tirupattur districts of Tamil Nadu. A strain of S. frugiperda nucleopolyhedrovirus (SpfrNPV NBAIR1) infecting S. frugiperda was isolated from the diseased larvae; morphological and biological characteristics were studied. Electron microscopic studies showed tetrahedral-shaped SpfrNPV occlusion bodies (OBs) of size 1.64 μm. Dose–mortality bioassays revealed that first, second and third instar larvae were equally susceptible (LC50 3.71–5.02 OBs/mm2) to SpfrNPV infection. A PCR technique for detection of viral DNA in S. frugiperda NPV was developed by employing the polyhedrin gene (polh)-specific primers. The amplicon of 618 bp was amplified, sequenced and NCBI GenBank accession number was obtained (MT422725). Blast analysis revealed that SpfrNPV conserved polh gene sequence matched 100% with the reference GenBank sequence (J04333) from the NCBI database which confirmed the identity of the SpfrNPV.Keywords
Insect Pests, Maize, Nucleopolyhedrovirus, Spodoptera frugiperda.- Cross-resistance and biochemical mechanism in an insecticide-resistant population of Trichogramma chilonis Ishii (Hymenoptera: Trichogrammatidae) and its parasitizing efficiency against invasive fall armyworm Spodoptera frugiperda (J.E. Smith)
Abstract Views :135 |
PDF Views:90
Authors
Priyanka Dupatne
1,
T. Venkatesan
2,
Omprakash Navik
3,
M. Mohan
3,
K. M. Venugopal
3,
Basavaarya
3,
V. Linga
3,
Y. Lalitha
3,
G. Sivakumar
3,
M. Ashwini
1
Affiliations
1 Department of Entomology, University of Agricultural Sciences, Gandhi Krishi Vignan Kendra, Bellary Road, Bengaluru 560 065, India, IN
2 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, India, IN
3 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, India, IN
1 Department of Entomology, University of Agricultural Sciences, Gandhi Krishi Vignan Kendra, Bellary Road, Bengaluru 560 065, India, IN
2 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, India, IN
3 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, India, IN
Source
Current Science, Vol 124, No 1 (2023), Pagination: 115-122Abstract
Trichogramma chilonis is an egg parasitoid of lepidopteran pests and widely used in biological control and integrated pest management (IPM) programmes. In this study, the cross-resistance in multiple insecticide-tolerant strain of T. chilonis was evaluated against chlorantraniliprole 18.5% SC, spinetoram 11.7% SC and thiamethoxam 12.6% + lambda-cyhalothrin 9.5% ZC. Bioassay studies revealed the highest resistance level against chlorantraniliprole (8.83-fold resistance) over the susceptible population, followed by spinetoram (2.41-fold). Metabolic enzymes carboxylesterase and glutathione S-transferase showed major involvement in the resistant populations, with the highest activity observed against chlorantraniliprole, followed by spinetoram. The resistant population at field recommended doses of chlorantraniliprole (400 ppm), parasitized 52.92% and 44.10% of Corcyra cephalonica and Spodoptera frugiperda eggs respectively, compared to 15.48% and 9.6% parasitism by the susceptible population. Integration and utilization of resistant strains of T. chilonis in IPM programmes can provide improved control of insect pests under insecticide-sprayed conditions and may reduce the insecticide load on cropsReferences
- Zang, L.-S., Wang, S., Zhang, F. and Desneux, N., Biological control with Trichogramma in China: history, present status and perspec-tives. Annu. Rev. Entomol., 2020, 66(1), 463–484.
- Li, L.-Y., Worldwide use of Trichogramma for biological control on different crops: a survey. In Biological Control with Egg Para-sitoids (eds Wajnberg, E. and Hassan, S. A.), CAB International, Oxon, UK, 1994, pp. 37–53.
- Parra, J. R. P. and Coelho Jr, A., Insect rearing techniques for bio-logical control programs, a component of sustainable agriculture in Brazil. Insects, 2022, 13, 105.
- Khanh, D. T., Chailleux, H., Tiradon, A., Desneux, N., Colombel, E. and Tabone. E., Using new egg parasitoids (Trichogramma spp.) to improve integrated management against Tuta absoluta. EPPO Bull., 2012, 42, 249–254.
- Shylesha, A. N. et al., Studies on new invasive pest Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae) and its natural enemies. J. Biol. Control, 2018, 32, 145–151.
- Ganiger, P. C., Yeshwanth, H. M., Muralimohan, K., Vinay, N., Kumar, A. R. V. and Chandrashekara, K., Occurrence of the new invasive pest, fall armyworm, Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae), in the maize fields of Karnataka, India. Curr. Sci., 2018, 115(4), 621–623.
- Sharanabasappa, et al., First report of the fall armyworm, Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae), an alien invasive pest on maize in India. Pest Manage. Hortic. Ecosyst., 2018, 24, 23– 29.
- Sisay, B., Tefera, T., Wakgari, M., Ayalew, G. and Mendesil, E., The efficacy of selected synthetic insecticides and botanicals against fall armyworm, Spodoptera frugiperda, in maize. Insects. 2019, 10(2), 45.
- Navik, O., Shylesha, A. N., Patil, J., Venkatesan, T., Lalitha, Y. and Ashika, T. R., Damage, distribution and natural enemies of invasive fall armyworm Spodoptera frugiperda (J.E. Smith) under rainfed maize in Karnataka, India. Crop Prot., 2021, 143, 105536.
- Visalakshi, M. et al., Report of the invasive fall armyworm, Spodo-ptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae) and its natural enemies on maize and other crops from Andhra Pradesh, India. J. Entomol. Zool. Stud., 2019, 7(4), 1348–1352.
- Sharanabasappa, D., Pavithra, H. B., Kalleshwaraswamy, C. M., Shivanna, B. K., Maruthi, M. S. and Mota-Sanchez. D., Field efficacy of insecticides for management of invasive fall armyworm, Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae) on maize in India. Fla. Entomol., 2020, 103(2), 221–227.
- Venkatesan, T. and Jalali, S. K., Trichogrammatids: adaptation to stresses. In Biological Control of Insect Pests using Egg Parasitoids (eds Sithanantham, S. et al.). Springer India, New Delhi, 2013, pp. 105–125.
- Jalali, S. K., Venkatesan, T., Srinivasa Murthy, K. and Ojha, R., Management of Helicoverpa armigera (Hübner) on tomato using insecticide resistance egg parasitoid, Trichogramma chilonis Ishii in farmers’ field. Indian J. Hortic. 2016, 73(4), 611–614.
- Panini, M., Manicard, G. C., Moores, G. and Mazzoni, E., An overview of the main pathways of metabolic resistance in insects. Invertebr. Surviv. J., 2016, 13(1), 326–335.
- Ye, M. et al., The role of insect cytochrome P450s in mediating in-secticide resistance. Agriculture, 2022, 12, 53.
- Oakeshott, J. G., Claudianos, C., Campbell, P. M., Newcomb, R. D. and Russell, J. R., Biochemical genetics and genomics of insect esterases. In Comprehensive Molecular Insect Science (eds Gilbert, L. I., Iatro, K. and Gill, S.), Elsevier, The Netherlands, 2010, pp. 1–73.
- Kliot, A. and Ghanim, M., Fitness costs associated with insecticide resistance. Pest Manage. Sci., 2012, 68(11), 1431–1437.
- Nagaraja, H., Mass production of Trichogrammatid parasitoids. In Biological Control of Insect Pests using Egg Parasitoids (eds Sithanantham, S. et al.), Springer, New Delhi, 2013, pp. 175–189.
- Ballal, C. R., Kumar, P. and Ramani, S., Laboratory evaluation, storability and economics of an artificial diet for rearing Chilo par-tellus (Swinhoe) (Lepidoptera: Pyralidae). J. Entomol. Res., 1995, 19, 135–141.
- Kerima, O. Z., Niranjana, P., Lalitha, Y., Jalali, S. K. and Ballal, C. R., Inheritance of monocrotophos resistance in egg parasitoid Tricho-gramma chilonis (Ishii) (Hymenoptera: Trichogrammatidae). Curr. Agric. Res. J., 2017, 5(3), 297–304.
- Bradford, M. M., A rapid and sensitive method for the quantification of microgram quantities of protein utilizing the principle of protein-dye binding. Anal. Biochem., 1976, 74, 248–254.
- Van Asperen, K., A study of housefly esterases by means of a sen-sitive colorimetric method. J. Insect Physiol., 1962, 8, 401–416.
- Kinoshita, F. K., Frawley, J. P. and Du Bois, K. P., Quantitative measurement of induction of hepatic microsomal enzymes by various dietary levels of DDT and toxaphene in rats. Toxicol. Appl. Phar-macol., 1966, 9, 505–513.
- Saber, M., Acute and population level toxicity of imidacloprid and fenpyroximate on an important egg parasitoid, Trichogramma cacoeciae (Hymenoptera: Trichogrammatidae). Ecotoxicology, 2011, 20, 1476– 1484.
- Preetha, G., Stanley, J., Suresh, S. and Kuttalam, S., Toxicity of selected insecticides to Trichogramma chilonis: assessing their safety in the rice ecosystem. Phytoparasitica, 2009, 37(3), 208–215.
- Yang, Y., Wang, C., Xu, H., Tian, J. and Lu, Z., Response of Tricho-gramma spp. (Hymenoptera: Trichogrammatidae) to insecticides at concentrations sublethal to Cnaphalocrocis medinalis (Lepidoptera: Pyralidae). J. Econ. Entomol., 2020, 113(2), 646–653.
- Xie, L. C., Jin, L. H., Lu, Y. H., Xu, H. X., Zang, L. S., Tian, J. C. and Lu, Z. X., Resistance of lepidopteran egg parasitoids, Tricho-gramma japonicum and Trichogramma chilonis, to insecticides used for control of rice planthoppers. J. Econ. Entomol., 2022, 115(2), 446–454.
- Shankarganesh, K., Paul, B. and Gautam, R. D., Studies on ecological safety of insecticides to egg parasitoids Trichogramma chilonis Ishii and Trichogramma brasiliensis (Ashmead). Natl. Acad. Sci. Lett., 2013, 36(6), 581–585.
- Larson, J. L., Redmond, C. and Potter, D. A., Comparative impact of an anthranilic diamide and other insecticidal chemistries on benefi-cial invertebrates and ecosystem services in turfgrass. Pest Manage. Sci., 2011, 68(5), 740–748.
- Ashwini, M., Mohan, M., Sivakumar, G. and Venkatesan, T., Enhanced insecticide-resistance spectrum in green lacewing predator, Chrys-operla zastrowi sillemi (strain PTS-8) and its potential role in the management of sucking pests of cotton. Curr. Sci., 2021, 120(2), 423–428.
- Khan, M. A., Lethal and parasitism effects of selected novel pesticides on adult Trichogramma chilonis (Hymenoptera: Trichogrammatidae). J. Plant Dis. Prot., 2020,127, 81–90.
- Deshmukh, Y. V., Undirwade, D. B. and Dadmal, S. M., Effect of some newer insecticides on parasitization by Trichogramma species under laboratory condition. J. Entomol. Zool. Stud., 2018, 6(3), 228– 231.
- Khan, M. A., Khan, H. and Ruberson, J. R., Lethal and behavioral effects of selected novel pesticides on adults of Trichogramma pre-tiosum (Hymenoptera: Trichogrammatidae). Pest Manage. Sci., 2015, 71, 1640–1648.
- Zhang, J., Du, W., Jin, X., Ruan, C. and Zang, L., Susceptibility of the egg parasitoid Trichogramma dendrolimi (Hymenoptera: Trichogrammatidae) to three kinds of insecticides commonly used in fields. Acta Phytophyl. Sin., 2014, 41, 555–561.
- Costa, M. A., Moscardini, V. F., da Costa Gontijo, P., Carvalho, G. A., de Oliveira, R. L. and de Oliveira, H. N., Sublethal and trans-generational effects of insecticides in developing Trichogramma galloi (Hymenoptera: Trichogrammatidae): toxicity of insecticides to Trichogramma galloi. Ecotoxicology, 2014, 23(8), 1399–1408.
- Jalali, S. K., Singh, S. P., Venkatesan, T. and Murthy, K. S., Develop-ment of endosulfan tolerant strain of an egg parasitoid Tricho-gramma chilonis Ishii (Hymenoptera: Trichogrammatidae). Indian J. Exp. Biol., 2006, 44(2), 584–590.