- Murthy K. Srinivasa
- R. Rajeshwari
- Nesil Liz Baby
- K. P. Dhanya
- Madhusmita Panda
- S. K. Jalali
- N. K. Krishna Kumar
- R. Gandhi Gracy
- M. Nagesh
- A. N. Shylesha
- R. J. Rabindra
- B. N. Hemalatha
- S. Sriram
- B. Reetha
- K. Srinivasa Murthy
- G. Ashok Kumar
- T. V. Baskaran
- P. Niranjana
- S. L. Ramya
- Ankita Gupta
- H. M. Yeshwanth
- Christer Hansson
- J. Poorani
- K. S. Murthy
- Y. Lalitha
- K. R. Lyla
- S.
- K. Srinivasamurthy
- C. Bharathi Dasan
- P. S. Devi
- N. S. Rao
- Arun Baitha
- S. P. Singh
- Sunil Joshi
- S. Joshi
- K. Selvaraj
- R. Sundararaj
- Chandish R. Ballal
- H. K. Mrudula
- S. Helen Mahiba
- M. Prathibha
- R. P. More
- Omprakash Navik
- Rakshit Ojha
- Srimoyee Basu
- K. Chandra
- Richa Varshney
- Pradeeksha Shetty
- Prabhu C. Ganiger
- K. Subaharan
- N. Bakthavatsalam
- A. Raghavendra
- T. R. Ashika
- V. Abdul Rasheed
- S. R. Koteswara Rao
- K. Sreedevi
- B. Bhaskar
- M. S. Abhishek
- B. C. Hanumanthaswamy
A B C D E F G H I J K L M N O P Q R S T U V W X Y Z All
Venkatesan, T.
- Detection and Characterization of Wolbachia in Cotesia plutellae (Kurdjumov) (Hymenoptera: Braconidae), a Parasitoid of the Diamond Back Moth Plutella xylostella (Linn.)
Authors
1 National Bureau of Agriculturally Important Insects, Post Bag No. 2491, H. A. Farm Post, Bellary Road, Bangalore, 560024, Karnataka, IN
Source
Journal of Biological Control, Vol 25, No 3 (2011), Pagination: 213-216Abstract
Cotesia plutellae (Kurdjumov) is an indigenous, larval endoparasitoid that attacks mid instar larvae of the diamond back moth (DBM). Although the parasitoid is distributed widely, not all local populations appear to be equally effective in controlling the DBM. Bacterial endosymbionts may play regulatory role in determining their efficiency. Field collected C. plutellae populations from cauliflower fields were assessed for the prevalence of the bacterial endosymbionts. Bacterial endosymbionts in the genus Wolbachia were detected in the populations obtained from Hoskote (Karnataka) and Thirupathi (Andhra Pradesh). PCR amplification using specific primers for Wolbachia revealed 528 and 518 bp for the populations, respectively. Sequencing of the Wolbachia surface protein, wsp, revealed Wolbachia infection to be related to Wolbachia endosymbiont of Cotesia glomerata outer surface protein, wsp gene (Genbank Accession No. AB094202) with maximum identity of 99% with BLAST search of NCBI. The sequence was submitted to the GenBank with the Accession No. JF421566. The detection of Wolbachia in the parasitoid signifying its role in biological manipulations of the parasitoid for enhanced efficiency is discussed.Keywords
Wolbachia, Characterization, Cotesia plutellae, Cabbage, Plutella xylostella.References
- Brand, A. M., Van Dijken, M. J., Kole, M. and Van Lenteren, J. C. 1984. Host-age and host-species selection of three species of Trichogramma evanescens Westwood, an egg parasite of several lepidopteran species, Meded Fak Landbouww Rijksuniversity de Genetics, 49: 839–847.
- Consoli, F. L. and Elliot, W. K. 2006. Symbiofauna associated with the reproductive system of Cotesia flavipes and Doryctobracon areolatus (Hymenoptera: Braconidae). Brazilian Journal of Morphological Sciences, 23: 463–470.
- Delgado, A. M. and Cook, J. M. 2009. Effects of a sex ratio distorting endosymbiont on mtDNA variation in a global insect pest. BMC Evolutionary biology, 9: 9–49.
- Doutt, R. D. 1958. The biology of parasitic Hymenoptera. Annual Review of Entomology, 4: 161–182.
- Huigens, M. E., Luck, R. F., Klaassen, R. H. G., Maas, M. F. P. M., Timmermans, M. J. T. N. and Stouthamer, R. 2000. Infectious parthenogenesis. Nature, 405, 178–179.
- Hosokawa, T., Kikuchi, Y., Shimada, M. and Fukatsu, T. 2006. Strict host symbiont co-speciation and reductive genome evolution in Insect gut bacteria. Plos Biology, 4 (10): 337–345
- Kokoza, V. A., Ahmed, W. L., Cho, N. Jasinskiene, A.A.J., and A. Raikhel. 2000. Engineering blood meal activated systemic immunity in the yellow fever mosquito, Aedes aegyptii. Proceedings of the National Academy of Sciences, USA, 97: 9144–49.
- Kevin, D. F., George, K., Kyei-Poku and Paul, C. C. 2006. Overview and relevance of Wolbachia bacteria in biocontrol research. Biocontrol Science & Technology, 16 : 767–788.
- Mochiah, M. B., Ngi-Song, A. J., Overholt, W. A. and Stouthamer, R. 2002. Wolbachia infection in Cotesia sesamiae (Hymeoptera: Braconidae) causes cytoplasmic incompatability: implications for biological control. Biological Control, 25 : 74–80.
- Mandrioli, M. 2009. The interaction insect-symbiont, rather than insect-pathogen, may open new perspectives in the understanding of the host choice in bacteria. Invertebrate Survival Journal, 6: 98–101.
- Ngi-Song, A. J. and Mochiah, M. B. 2001. Polymorphism for Wolbachia infections in Eastern and Southern African Cotesia sesamiae (Cameron) (Hymenoptera: Braconidae) populations. Insect Science and its Application, 21: 369–374.
- Pidiyar, V. J., Jangid, K., Patole, M. S. and Shouche, Y. S. 2003. Detection and phylogenetic affiliation of Wolbachia sp. from Indian mosquitoes Culex quinquefasciatus and Aedes albopictus. Current Science, 84: 1136–1139.
- Shoemaker, D. D., Machado, C. A., Molbo, D., Werren, J. H., Windsor, D. M. and Herre, E. A. 2002. The distribution of Wolbachia in wasps: correlations with host phylogeny, ecology and population structure. Proceedings of the Royal Society, London B, 269: 2257–2267.
- Trumble J. T. and Alvarado-Rodriguez, B. 1998. Trichogrammatid egg parasitoids in the management of vegetable-crop insect pests. In: R. L. Ridgway, M. P. Hoffmann, M. N. Inscoe and C. S. Glenister, (eds). Mass-Reared Natural Enemies: Application, Regulation, and Needs. Thomas Say Publications in Entomology, Entomological Society of America, Lanham, MD, USA, pp 158–184.
- Weeks, A. R., Reynolds, K. T., Hoffmann, A. A. and Mann, H. 2002. Wolbachia dynamics and host effects. Trends in Ecology and Evolution, 17: 257–262.
- Werren, J. H. and Windsor, D. M. 2000. Wolbachia infection frequencies in insects: evidence of a global equilibrium. Proceedings of the Royal Society, London B., 267: 1277–1285.
- In silico Docking Studies on Cytochrome P450 Enzymes of Helicoverpa armigera (Hubner) and Trichogramma cacoeciae Marchal and Implications for Insecticide Detoxification
Authors
1 Molecular Entomology Laboratory, National Bureau of Agriculturally Important Insects, Post Bag No. 2491, H. A. Farm Post, Bellary Road, Hebbal, Bangalore 560 024, Karnataka, IN
Source
Journal of Biological Control, Vol 27, No 1 (2013), Pagination: 1-9Abstract
In silico docking of cytochrome P450 monooxygenase (CYP450) of an insect, Helicoverpa armigera (Hübner) and a parasitoid, Trichogramma cacoeciae Marchal was studied with two insecticides, monocrotophos and fenvalerate. The CYP450 sequences of H. armigera (CYP9A12), T. cacoeciae (CYP4G12) and a human microsomal sequence CYP3A4, as positive control were retrieved from NCBI’s GenBank database. The structure, as predicted by SOPMA, of CYP450 in H. armigera contained 78.7% helix and 43.3% sheets, while that of T. cacoeciae contained 60.6% helix and 68.5% sheets. The three-dimensional molecular models of CYP450 of H. armigera and T. cacoeciae indicated that 96.5 and 97.2% residues, respectively, were in the most favored region. The docking studies revealed that the binding energy of H. armigera was -3.50 and -7.65 kcal/mole compared to the binding energy of T. cacoeciae -2.96 and -5.28 kcal/mole for monocrotophos and fenvalerate, respectively, inferring stronger interaction of H. armigera CYP450 with the insecticides and thereby higher potential for resistance in H. armigera.Keywords
Cytochrome P450, Helicoverpa armigera, Trichogramma cacoeciae, In silico Molecular Docking.References
- Armes NJ, Jadhav DR, DeSouza KR. 1996. A survey of insecticides resistance in Helicoverpa armigera in the Indian subcontinent. Bull Ent Res. 86: 499–514.
- Bachar O, Fischer D, Nussinov R, Wolfson HJ. 1993. A Computer vision based technique for 3-D sequence independent structural comparison of proteins. Protein Eng. 6: 279–288.
- Baudry J, Li W, Pan L, Berenbaum MR, Schuler MA. 2003. Molecular docking of substrates and inhibitors in the catalytic site of CYP6B1, an insect cytochrome P450 monooxygenase. Protein Eng. 16: 577–587.
- Baudry J, Rupasinghe S, Shuler MA. 2006. Classdependent sequence alignment strategy improves the structural and functional modeling of P450s. Protein Eng Des Sel. 19: 345–353.
- Bikadi Z, Hazai E. 2009. Application of the PM6 semiempirical method to modeling proteins enhances docking accuracy of AutoDock. J Cheminf. 1: 15.
- Bull DL, House VS. 1983. Effects of different insecticides on parasitism of host eggs by Trichogramma pretiosum Riley. Southwestern Entomol. 8: 46–53.
- Cariño FA, Koener JF, Plapp Jr. FW, Feyereisen R. 1994. Constitutive over expression of the cytochrome P450 gene CYP6A1 in a house fly strain with metabolic resistance to insecticides. Insect Biochem Mol Biol. 24: 411–418.
- Daborn PJ, Yen JL, Bogwitz MR, Le Goff G, Feil E, Jeffers S. 2002. A single p450 allele associated with insecticide resistance in Drosophila. Science 297: 2253–2256.
- Daborn PJ, Lumb C, Boey A, Wong W, ffrench-Constant RH, Batterham P. 2007. Evaluating the insecticide resistance potential of eight Drosophila melanogaster cytochrome P450 genes by transgenic overexpression. Insect Biochem Mol Biol. 37: 512–519.
- de Graaf C, Vermeulen NP, Feenstra KA. 2005. Cytochrome P450 insilico: an integrative modeling approach. J Med Chem. 48: 2725–2755.
- Edgar RC. 2004. MUSCLE: multiple sequence alignment with high accuracy and high throughput. Nucleic Acids Res. 32, 1792–1797.
- Feyereisen R, Insect P450 enzymes, Ann Rev Entomol. 44: 507–733.
- Jalali SK, Singh SP, Venkatesan T, Murthy KS, Lalitha Y. 2006. Development of endosulfan tolerant strain of an egg parasitoid Trichogramma chilonis Ishii (Hymenoptera: Trichogrammatidae). Indian J Exp Biol. 44: 584–590.
- Jones RT, Bakker SE, Stone D, Shuttleworth SN, Boundy S, McCart C, Daborn PJ, ffrench-Constant RH, van den Elsen JM. 2010. Homology modelling of Drosophila cytochrome P450 enzymes associated with insecticide resistance. Pest Mgmt Sci. 66: 1106–1115.
- Korytko PJ, Scott JG. 1998. CYP6D1 protects thoracic ganglia of houseflies from the neurotoxic insecticide cypermethrin. Arch Insect Biochem Physiol. 37: 57–63.
- Kranthi KR, Jadhav DR, Kranthi S, Wanjari RR, Ali SS, Russell DA. 2002. Insecticide resistance in five major insect pests of cotton in India. Crop Prot. 21: 449-460.
- Laskowski RA, MacArthur MW, Moss DS, Thornton JM. 1993. PROCHECK: a program to check the stereochemical quality of protein structures. J Appl Cryst. 26: 283-291.
- Li LY. 1994. Worldwide use of Trichogramma for biological control on different crops: a survey. In: Wajnberg, E. and Hassan, SA. (Eds.), Biological control with egg parasitoids, CAB International, Wallingford, UK, pp. 37–44.
- Liu N, Scott JG. 1998. Increased transcription of CYP6D1 causes cytochrome P450-mediated insecticide resistance in house fly. Insect Biochem Mol Biol. 28: 531–535.
- Lopez JD, Morrison RK. 1985. Parasitization of Heliothis spp. eggs after augmentative releases of Trichogramma pretiosum Riley. Southwestern Entomol. 8: 110–138.
- Maitra S, Dombrowski SM, Waters LC, Ganguly R. 1996. Three second chromosome-linked clustered Cyp6 genes show differential constitutive and barbitalinduced expression in DDT-resistant and susceptible strains of Drosophila melanogaster. Gene 180: 165–171.
- Morris GM, Goodsell DS, Halliday RS, Huey R, Hart WE, Belew RK, Olson AJ. 1998. Automated docking using a Lamarckian genetic algorithm and an empirical binding free energy function. J Comp Chem. 19: 1639–1662.
- Panigrahi SK. 2008. Strong and weak hydrogen bonds in protein-ligand complexes of kinases: a comparative study. Amino Acids 34: 617–633.
- Patil R, Das S, Stanley A, Yadav L, Sudhakar A, Varma AK. 2010. Optimized hydrophobic interactions and hydrogen bonding at the target-ligand interface leads the pathways of drug-designing. PLoS One 5: e12029.
- Pedra JHF, Mclntyre LM, Scharf ME, Pittendrigh BR. 2004. Genome-wide transcription profile of field and laboratory-selected dichlorodiphenyltrichloroethane (DDT)-resistant Drosophila. Proc Nat Acad Sci USA. 101: 7034–7039.
- Pittendrigh B, Aronstein K, Zinkovsky E, Andreev O, Campbell B, Daly J, Trowell S, ffrench-Constant RH. 1997. Cytochrome P450 genes from Helicoverpa armigera: expression in a pyrethroid – susceptible and – resistant strain. Insect Biochem Mol Biol. 27: 507–512.
- Ramachandran GN, Ramakrishnan C, Sasisekharan V. 1963. Stereochemistry of polypeptide chain configurations. J Mol Biol. 7: 95–99.
- Ranson H, Jensen B, Vulule JM, Wang X, Hemingway J, Collins FH. 2000a. Identification of a point mutation in the voltage-gated sodium channel gene of Kenyan Anopheles gambiae associated with resistance to DDT and pyrethroids. Insect Mol Biol. 9: 491–497.
- Ranson H, Jensen B, Wang X, Prapanthadara L, Hemingway J, Collins FH. 2000b. Genetic mapping of two loci affecting DDT resistance in the malaria vector Anopheles gambiae. Insect Mol Biol. 9: 499–507.
- Rocher A, Marchand-Geneste N. 2008. Homology modeling of the Apis melifera nicotinic acetylcholine receptor (nAChR) and docking of imidacloprid and fipronil insecticides and their metabolites. SAR and QSAR in Environ Res. 19: 245–261.
- Sabourault C, Guzov VM, Koener JF, Claudianos C, Plapp Jr. FW, Feyereisen R. 2001. Overproduction of a P450 that metabolizes diazinon is linked to a loss of function in the chromosome 2 ali-esterase (MdalphaE7) gene in resistant house flies. Insect Mol Biol. 10: 609–618.
- Scott JG. 1999. Cytochromes P450 and insecticide resistance. Insect Biochem Mol Biol. 29: 757–777.
- Shen J, Wu Y. 1995. Resistance to Helicoverpa armigera to insecticides and its management. China Agricultural Press, Beijing, China, pp. 1–88.
- Solis FJ, Wets R.J-B. 1998. Minimization by random search techniques. Maths Operation Res. 6: 19–30.
- Tares S, Berge JB, Amichot M. 2000. Cloning and expression of cytochrome P450 genes belonging to the CYP4 family and to a novel Family, CYP48, in two hymenopteran insects, Trichogramma cacoeciae and Apis mellifera. Biochem Biophys Re. Commun. 268: 677–682.
- Wheelock GD, Scott JG. 1992. Anti-P450I pr antiserum inhibits specific monooxygenase activities in LPR housefly microsomes. J Exp Zool. 264: 153–158.
- Yang Y, Yue L, Chen S, Wu Y. 2008. Functional expression of Helicoverpa armigera CYP912 and CYP9A14 in Saccharomyces cerevisiae. Pesticide Biochem Physiol. 92: 101–105.
- Yano JK, Wester MR, Schoch GA, Griffin KJ, Stout CD, Johnson EF. 2004. The structure of human microsomal cytochrome P450 3A4 determined by X-ray crystallography to 2.05A° resolution. J Biol Chem. 279: 38091–38094.
- Characterization and Identification of Acerophagus papayae Noyes and Schauff (Hymenoptera: Encyrtidae), an Introduced Parasitoid of Papaya Mealybug, Paracoccus marginatus Williams and Granara De Willink through DNA Barcode
Authors
1 National Bureau of Agriculturally Important Insects, P.B. No. 2491, H.A. Farm Post, Hebbal, Bangalore 560 024, Karnataka, IN
Source
Journal of Biological Control, Vol 25, No 1 (2011), Pagination: 11–13Abstract
The papaya mealybug, Paracoccus marginatus Williams and Granara de Willink, is a serious invasive pest in India and causes severe yield loss. Acerophagus papayae Noyes and Schauff (Encyrtidae) is one of the efficient parasitoids for the suppression of papaya mealybug in its native range. This parasitoid was introduced from Puerto Rico in 2010 through USDA-APHIS for use against the papaya mealybug. Subsequently, natural occurrence of the parasitoid was observed in mealybug infested papaya fields at Pune and the parasitoid was identified as A. papayae based on morphology based taxonomy at NBAII. The study was undertaken for the DNA barcoding of A. papayae, using CO1 region in order to supplement and confirm that the introduced and Pune populations belonged to the same species and the study revealed that the A. papayae populations from Pune and USA are one and the same having fragment size of ~673bp.Keywords
Papaya Mealybug, Paracoccus Marginatus, Acerophagus Papayaa, Cytochrome C Oxidase-I (CO1), DNA Barcode.References
- Amarasekare, K. G., Mannion, C. M. and Epsky, N. D. 2009. Efficiency and establishment of three introduced parasitoids of the mealybug Paracoccus marginatus (Hemiptera: Pseudococcidae). Biological Control, 51: 91–95.
- Avise, J.C. 2000. Phylogeography. The history and formation of species. Cambridge, MA; Harvard University Press.
- Folmer, O., Black, M., Howh, W., Lutz, R. and Vrijenhoek, R. 1994. DNA primer for amplification of mitochondrial cytochrome c oxidase subunit I from diverse metazoan invertebrates. Molecular Marine Biology and Biotechnology, 3: 294–299.
- Greenstone, M. H., Rowley, D. L., Heimbach, U., Lundgren, J. G., Pfannenstiel, R. S. and Rehner, S. A. 2005. Barcoding generalist predators by polymerase chain reaction: Carabids and spiders. Molecular Ecology, 14: 3247–3266.
- Hebert, P. D. N., Penton, E. H., Burns, J. M., Janzen, D. H. and Hallwachs, W. 2004. Ten species in one: DNA barcoding reveals cryptic species in the neotropical skipper butterfly, Astraptes fulgerator. Proceedings of the National Academy of Sciences, USA, 101: 14812–14817.
- Kim, J.M., Yoon, J.H., Im, H.H., Jeong, U.H., Kim, I.M., Kim, R.S. and Kim, I. 2009. Mitochondrial sequence variation of the bumblebee, Bombus ardens (Hymenoptera: Apidae). Journal of Asia-Pacific Entomology, 12: 133–139.
- Kumar, N. P., Rajavel, A. R., Natarajan, R. and Jambulingam, P. 2007. DNA barcodes can distinguish species of Indian mosquitoes (Diptera: Culicidae). Journal of Medical Entomology, 44: 1–7.
- Miller, J. S., Brower, A. V. Z. and Desalle, R. 1997. Phylogeny of the neotropical moth tribe Josini (Notodontidae: Dioptinae): Comparing and combining evidence from DNA sequences and morphology. Biological Journal of the Linnean Society, 60: 297–316.
- Muniappan, R., Meyerdirk, D. E., Sengebau, F. M., Berringer, D. D. and Reddy, G. V. P. 2006. Classical biological control of papaya mealybug (Hemiptera: Pseudococcidae) in the Republic of Palau. Florida Entomologist, 89: 212–217.
- Pokharkar, D. S., Nakat, R. V., Tamboli, N. D., Dhane, A. S., Jadhav, S. S., Chandele, A. G. and Rabindra, R. J. 2010. A new record of Acerophagus papayae Noyes and Schauff on papaya mealybug, Paracoccus marginatus Williams and Granara de Willink, in Pune region of Maharashtra state. Journal of Biological Control, 24: 291.
- Ratnasingham, S. and Hebert, P. D. N. 2007. BOLD: The Barcode of Life Data System (www. Barcodinglife.org). Molecular Ecology Notes, 7: 355–364.
- Shylesha, A. N., Joshi, S., Rabindra, R. J. and Bhumannavar, B. S. 2010. Classical biological control of the papaya mealybug. Newsletter, NBAII, Bangalore, India.
- Smith, M. A., Rodriguez, J., Whitefield, J., Deans, A., Janzen, D. H., Hallwachs, W. and Hebert, P. D. N. 2008. Extraordinary diversity of parasitoid wasps exposed by iterative integration of natural history, DNA barcoding, morphology and collections. Proceedings of the National Academy of Sciences USA, 105: 12359–12364.
- Tanwar, R. K., Jeyakumar, P. and Vennila, S. 2010. Papaya mealybug and its management strategies. Technical Bulletin 22, NCIPM, New Delhi, India, 22 pp.
- Walsh, P. S., Metzger, D. A. and Higuchi, R.1991. Chelex 100 as a medium for simple extraction of DNA for PCRbased typing from forensic material. Biotechniques, 10: 506–513.
- Molecular Identification of Yeast Like Microorganisms Associated with Field Populations of Aphid Predator, Chrysoperla zastrowi sillemi (Esben-Petersen) (Neuroptera: Chrysopidae) and Their Role in Fecundity
Authors
1 National Bureau of Agriculturally Important Insects, H.A. Farm Post, Hebbal, Bangalore-560024, IN
Source
Journal of Biological Control, Vol 27, No 3 (2013), Pagination: 176–183Abstract
Resident microflora of alimentary canal and fat bodies associated with eleven field collected Chrysoperla zastrowi sillemi (Esben-Petersen) adult females were characterized and their possible role in influencing the fecundity was studied. The isolated yeasts varied among different populations of the predator. Culturable yeasts viz., Wickerhamomyces anomalus, Pichia anomala, Candida blankii, C. apicola, C. pimensis, Torulaspora delbrueckii, Zygosaccharomyces rouxii and Kodamea ohmeri were isolated from gut, diverticulum and fat bodies of the adult females and characterized by biochemical and molecular tools. The yeast isolate of T. delbrueckii in combination with honey and castor pollen grains were found to increase the fecundity of the adult females as compared to those that were reared on honey and pollen in different generations.Keywords
Chrysoperla Zastrowi Sillemi, Yeast, Molecular Characterization, Fecundity.References
- Athan R, Kaydan B, Ozgokce MS. 2004. Feeding activity and life history characteristics of the generalist predator, Chrysoperla externa (Neuroptera: Chrysopidae) at different prey densities. J Pest Sci. 77 (1):17–21.
- Canard M, Semeria Y, New TRR. 1984. Biology of Chrysopidae, Dr. W. Junk, Publisher: The Haque, The Netherlands. 294.
- Canard M, Kokubu K, Duelli P. 1990. Tracheal trunks supplying air to the foregut and feeding habits in adults of European green lacewing species (Insecta: Neuroptera: Chrysopidae). Pretoria, Republic of South Africa: Dept of Agricultural Development; 277–286.
- Cohen AC. 1999. Artificial diet for rearing entomophages comprising sticky, cooked whole eggs (continuation in part). U.S. Patent. 51999; 945:271.
- Coppel HC, Mertins JW. 1977. Biological Insect Pest Suppression. Spinger-Verlag. Berlin, Germany.
- Fresitas S. 2002. Controle biológico no Brasil: parasitóides e predadores. São Paulo. Manole.
- Gibson CM, Hunter MS. 2005. Negative fitness consequences and transmission dynamics of a heritable fungal symbiont of a parasitic wasp. Appl Env Microbiol. 75:3115–3119.
- Hagen KS. 1950. Fecundity of Chrysopa californica as affected by synthetic foods. J Econ Ent. 43:101–104.
- Hagen KS, Tassan RL. 1966. The influence of protein hydrolysates of yeasts and chemically defined upon the fecundity of Chrysopa carnea (Neuroptera). Vestn Cesk Spol Zool. 30:219–227.
- Hagen KS, Tassan RL. 1972. Exploring nutritional roles of extracellular symbiotes on the reproduction of honeydews feeding adult chrysopids and tephritids p. 323–251. In: Insect and Mite Nutrition. Significance and Implications in Ecology and Pest Management.
- Hagen KS, Tassan RL, Sawall EF. 1970. Some ecophysiological relationships between certain Chrysopa, honeydews and yeasts. Boll Lab Entomol Agric Portici 28:113–134.
- Hassan SA. 1974. Mass-culturing and utilization of Chrysopa spp. (Neuroptera: Chrysopidae) in the control of insect pests. Zeitschrift fur Pflanzenkrankheiten und Pflanzenschutz 81:620–637.
- Henry CS, Brooks SJ, Johnson JB, Venkatesan T, Duelli P. 2010. The most important lacewing species in Indian agricultural crops, Chrysoperla sillemi (EsbenPetersen), is a subspecies of Chrysoperla zastrowi (Esben-Petersen) (Neuroptera: Chrysopidae). J Nat Hist. 44:2543–2555.
- Johnson JB. 1982. Bionomics of some symbiote using Chrysopidae (Insecta: Neuroptera) from the Western United States. Ph.D. dissertation. University of California, Nerkeley.
- Marchini D, Rosetto M, Dallai R, Marri, L. 2002. Bacteria associated with oesophageal bulb of the med fly Ceratitis capitata (Diptera: Tephritidae). Curr Microbiol. 44:120–124.
- McCormack PJ, Wildman HG, Jeffries P. 1994. Production of antibacterial compounds by phylloplane-inhabitating yeasts and yeast like fungi. App Env Microbiol. 60 (3):927–931.
- Nguyen NH, Suh SO, Erbil CK, Blackwell M. 2006. Metschnikowia noctiluminum sp. nov. Metschnikowia corniflorae sp. nov. and Candida chrysomelidarum sp. nov., isolated from green lacewings and beetles. Mycol Res. 110:346–356.
- Nguyen NH, Suh SO, Blackwell M. 2007. Five novel Candida species in insect- associated yeast clades isolated from Neuroptera and other insects. Mycologia 99:842–858.
- Peter W, Magali P, Elzbieta R, Paul GB, Stefanos A, Miryan C, Tobias, UTL, Lee JR, Arne H, Marie B, Cletus PK, Jure P, Alan K. 2012. This is not an Apple– Yeast Mutualism in Codling Moth. J Che Ecol. 38:949–957.
- Sayyed AH, Pathan AK, Faheem U. 2010. Cross-resistance, genetics and stability of resistance to deltamethrin in a population of Chrysoperla carnea from Multan, Pakistan. Pesticide Biochem Physiol. 98:325–332.
- Smith RC. 1922. The biology of the Chrysopidae. CornellUniv. Agr.
- Suh SO, Blackwell M. 2004. Metschnikowia chrysoperlae sp. nov., Candida picachoensis sp. nov. and Candida pimensis sp. nov., isolated from the green lacewings Chrysoperla comanche and Chrysoperla carnea (Neuroptera: Chrysopidae). Intl J Syst Evol Microbiol. 54:1883–1890.
- Tamura K. 1992. Estimation of the number of nucleotide substitutions when there are strong transition, transversion and GC content biases. Mol Biol Evol. 9:678–687.
- Tamura K, Peterson N, Stechar G, Nei M, Kumar S. 2011. MEGA. Molecular evolutionary genetic analysis using maximum likelihood, Mol Biol Evol. 38:2731–2739.
- Tauber MJ, Tauber CA, Daane KM, Hagen KS. 2000. Commercialization of predators: recent lessons from green lacewings (Neuroptera: Chrysopidae). Am Entomol. 46:26–38.
- Vega FE, Dowd PF. 2005. The role of yeasts as insect endosymbionts. Insect-Fungal Associations: ecology and evolution, New York: Oxford University Press, 211–243.
- Venkatesan T, Jalali SK, Murthy KS, Rabindra RJ, Lalitha Y. 2009. Occurrence of insecticide resistance in field populations of Chrysoperla zastrowi arabica (Neuroptera: Chrysopidae) in India. Indian J Agric Sci. 79:910–912.
- Woolfolk SW, Inglis GD. 2003. Microorganisms associated with field-collected Chrysoperla rufilabris (Neuroptera: Chrysopidae) adults with emphasis on yeast symbionts. Biol Control 29, 155–168.
- Woolfolk SW, Cohen AC, Inglis GD. 2004. Morphology of the alimentary canal of Chrysoperla rufilabris (Neuroptera: Chrysopidae) adults in relation to microbial symbionts. Ann Ent Soc Am. 97:795–808.
- Zacchi L, Vaughan Martini A. 2002. Yeats associated with insects in agricultural areas of Perugia Italy. Ann Microbiol. 52:237–244.
- Assessment of Genetic Variation in Cotesia flavipes Cameron (Hymenoptera: Braconidae) Populations as Revealed by Mitochondrial Cytochrome Oxidase Gene Sequences
Authors
1 National Bureau of Agriculturally Important Insects, Post Bag No. 2491, H. A. Farm Post, Bellary Road, Bangalore 560024, Karnataka, IN
Source
Journal of Biological Control, Vol 23, No 3 (2009), Pagination: 249-253Abstract
The cytochrome oxidase gene (COI) was employed to assess the genetic variation in different populations of Cotesia flavipes. Partial sequences of the COI gene for the populations from Bangalore, Hyderabad, New Delhi and Shimla were analyzed to assess the homology and the usefulness of this genetic region for phylogenetic studies. PCR using COI-F and COI-R primers amplified a product of approximately 550 bp which was similar for all the four populations. Populations were by and large similar in the COI gene sequenced and there was no variation with our sequences and those of sequences worldwide. The multiple alignments were performed for four populations which revealed similarity of the partial COI gene sequences. Comparative analysis of partial sequences of COI gene produced a phylogenetic tree. Phylogenetic analysis revealed that all our populations were in a single clade with high boot strap value, suggesting highest similarity.Keywords
Cotesia flavipes, Cytochrome Oxidase, Genetic Variation.References
- Altschul, S. F., Madden, T. L., Schaffer, A. A., Zhang, Z.,Miller, W. and Lipman, D. J. 1997. Gapped BLASTand PSI-BLAST: a new generation of protein database search programmes. Nucleic Acids Research,25: 3389–3402.
- Ballal, C. R.., Kumar, P. and Ramani, S. 1995. Laboratoryevaluation, storability and economics of anartificial diet for rearing Chilo partellus (Swinhoe)(Lepidoptera: Pyralidae). Journal of EntomologicalResearch, 19:135–141.
- Borah, B. K. and Arya, M. P. S.1995. Natural parasitisationof the sugarcane Plassey borer (Chilo tumidicostalisHmpsn.) by braconid larval parasitoid in Assam. Annals of Agricultural Research, 16 : 362–363.
- Dowton, M. and Austin, A. D. 1994. Simultaneousanalysis of 16S, 28S, CO1 and morphology in theHymenoptera: Apocrita-evolutionary transitionsamong parasitic wasps. Proceedings of NationalAcademy of Sciences, 91: 9911–9915.
- Fakrudin, B., Prakash, S. H., Krishnareddy, K. B.,Vijaykumar Badari Prasad, P. R., Patil, B. V. andKuruvinashetti, M. S. 2004. Genetic variation ofcotton bollworm, Helicoverpa armigera (Hubner)(Lepidoptera : Noctuidae) of South Indian cottonecosystem using RAPD markers. Current Science,87: 1654–1659.
- Felsenstein, J. 1985. Confidence limits on phylogenies:an approach using the bootstrap. Evolution, 39:783–791.
- Hoy, M. A. 1994. Insect Molecular Genetics: an Introductionto Principles and Applications. Academic Press,San Diego, CA, USA, 546pp.
- Kimura, M. 1980. A simple method for estimatingevolutionary rate of base substitutions throughcomparative studies of nucleotide sequences. Journal of Molecular Evolution, 16: 111–120.
- Kfir, R., Overholt, W. A., Khan, Z. R. and Polaszek, A. 2002. Biology and management of economicallyimportant lepidopteran cereal stem borers in Africa. Annual Review of Entomology, 47: 701–731.
- Kumar, S., Tamura, K. and Nei, M. 2004. MEGA 3:integrated software for molecular evolutionarygenetics analysis and sequence alignment. Briefings in Bioinformatics, 5: 150–163.
- Kankare, M., Stefanescu, C., Saskya, V. N. and Shaw, M. R. 2005. Host specialization by Cotesia wasps(Hymenoptera: Braconidae) parasitizing speciesrich Melitaeini (Lepidoptera: Nymphalidae)communities in north-eastern Spain. BiologicalJournal of the Linnean Society, 86: 45–65.
- Mohan, B. R., Verma, A. N. and Singh, S. P. 1991. Periodicparasitisation of Chilo partellus (Swinhoe) larvaeon forage sorghum in Haryana. Journal of InsectScience, 4: 167–169.
- Muirhead, K. A., Murphy, N. P., Sallam, M. N., Donnellan,S. C. and Austin, A.D. Mitochondrial DNAphylogeography of the Cotesia flavipes complexof parasitic wasps (Hymenoptera: Braconidae). Annals of the Entomological Society of America,42: 309–318.
- Potting, R. P. J.; Vet., L. E. M and Overholt, W. A.1997. Geographic variation in host selection behaviour and reproductive success in the stemborer parasitoid Cotesia flavipes (Hymenoptera:Braconidae). Bulletin of Entomological Research,87: 515–524.
- Rattan, R. S., Reineke, A., Ashok, H., Gupta, P. R. andZebitz, C. P. W. 2006. Molecular phylogeny ofCotesia species (Hymenoptera: Braconidae)inferred from a 16s gene. Current Science, 91:1460–1461.
- Scott, K. D., Wilkinson, K. S. and Merritt, M. A. 2003. Genetic shifts in Helicoverpa armigera (Hubner)(Lepidoptera: Noctuidae) over a year in theDawson/Callide valleys. Australian Journal ofAgricultural Research, 54: 739–744.
- Whitfield, J. B. 1997. Hierarchical analysis of variationin the mitochondrial 16S gene amongHymenoptera. Molecular Biology and Evolution, 15: 1728-1743.
- Influence of Parasitoid-Host Density on the Behaviour Ecology of Goniozus nephantidis (Muesebeck) (Hymenoptera: Bethylidae), a Parasitoid of Opisina arenosella Walker
Authors
1 National Bureau of Agriculturally Important Insects, Post Bag No. 2491, H. A. Farm Post, Hebbal, Bangalore 560024, Karnataka, IN
Source
Journal of Biological Control, Vol 23, No 3 (2009), Pagination: 255-264Abstract
Since Goniozus nephantidis (Muesebeck) is found to have strong parental care for its progeny, the influence of different densities of G. nephantidis and its host, Corcyra cephalonica (Stainton) on the behaviour ecology of the parasitoid was studied. Interaction between different densities of the host and parasitoid revealed that a ratio of 1:1 was significantly superior to all other ratios resulting in maximum parasitism (9.0 larvae / female), fecundity (93.2/female) and number of progenies (75.2/female). Exposing more than one C. cephalonica larva did not significantly increase the parasitizing efficiency, fecundity and progeny produced. Conversely, exposing a single C. cephalonica larva to several female parasitoids adversely affected the biological attributes of the parasitoid. Increasing the densities of either host insects or parasitoids had an inverse relationship with oviposition behaviour, parasitism efficiency and progeny production of the parasitoid establishing the important and significant role played by host-parasitoid density.Keywords
Corcyra cephalonica, Density, Goniozus nephantidis, Opisina arenosella, Parasitizing Behaviour, Parental Care.References
- Antony J. and Kurian, C. 1960. Studies on the habits and lifehistory of Perisierola (=Goniozus) nephantidisMuesebeck. Indian Coconut Journal, 13: 143–153.
- Batchelor, T. P., Hardy, I. C. W. and Barrera, J. F. 2006. Interactions among bethylid parasitoid speciesattacking the coffee berry borer, Hypothenemushampei (Coleoptera: Scolytidae). BiologicalControl, 36: 106–118.
- Batchelor, T. P., Hardy, I. C. W., Barrera, J. F. and Lachaud,G. P. 2005. Insect gladiators II: Competitiveinteractions within and between bethylidparasitoid species of the coffee berry borer,Hypothenemus hampei (Coleoptera: Scolytidae). Biological Control, 33: 194–202.
- Cock, M. J. W. and Perera, P. A. C. R. 1987. Biologicalcontrol of Opisina arenosella Walker(Lepidoptera: Oecophoridae). Biocontrol Newsand Information, 8: 283–309.
- Dharmaraju, E. 1963. Biological control of coconut leafcaterpillar (Nephantis serinopa Meyrick) inCeylon. Bulletin of Coconut Research Institute(Ceylon), 21, 46 pp.
- Doutt, R. L. 1973. Maternal care of immature progeny byparasitoids. Annals of the Entomological Societyof America, 66: 486–487.
- Eitarn, A. 2001. Oviposition behaviour and developmentof immature stages of Parasierola swirskiana, aparasitoid of lesser date moth. Phytoparasitica,29: 1–8.
- Enquist, M. and Leimar, O. 1990. The evolution of fatalfighting. Animal Behaviour, 39: 1–9.
- Field, S. A. and Calbert, G. 1998. Patch defense in theparasitoid wasp Trissolcus basalis: when tobegin fighting? Behaviour, 135: 629–642.
- George, S. A. and Abdurahiman, U. C. 1986. Some aspectsof the reproductive biology of Goniozus sp. (Hymenoptera: Bethylidae), as external parasiteof mango leaf webber, Lamida moncusalisWalker. National Seminar on Entomophagousinsects and other Arthropods, Calicut. Proceedings, pp. 110–115.
- Goertzen, R. and Doutt, L. R. 1975. The ovicidal propensityof Goniozus. Annals of the EntomologicalSociety of America, 68: 869–870.
- Gordh, G. 1976. Goniozus gallicola Fouts, aparasitoid of moth larvae with notes onother bethylids (Hymenoptera: Bethylidae: Lepidoptera: Gelechiidae)). USDA TechnicalBulletin No. 1524, 27p.
- Goubault, M., Batchelor, T. P., Linforth, R. S. T., Taylor, A.J. and Hardy, I. C. W. 2006. Volatile emissionby contest losers revealed by real–time chemicalanalysis. Proceedings of the Royal Society ofLondon, B 273: 2853–2859.
- Goubault, M., Mack, A. F. S. and Hardy, I. C. W. 2007a.Encountering competitors reduces clutch sizeand increases offspring size in a parasitoid withfemale-female fighting. Proceedings of the RoyalSociety of London, B 274: 2571–2577.
- Goubault, M., Scott, D., Hardy, I. C. W. 2007b. Theimportance of offspring value: maternal defensein parasitoid contests. Animal Behaviour,74: 437–446.
- Grafen, A. 1987. The logic of diversely asymmetric contestsrespectfor ownership and the desperado effect. Animal Behaviour, 35: 462–467.
- Green, R. F., Gordh, G. and Hawkins, B. A. 1982. Precisesex ratios in highly inbred parasitic wasps. American Naturalist, 120: 653–665.
- Griffiths, N. T. and Godfray, H. C. J. 1988. Local matecompetition, sex ratio and clutch size in bethylidwasps. Behavioural Ecology and Sociobiology,22: 211–217.
- Hamilton, W. D. 1967. Extraordinary sex ratios. Science,156: 477–488.
- Hammerstein, P. 1981. The role of asymmetrics in animalcontests. Animal Behaviour, 29: 193–205.
- Hardy, I. C. W. 1995. Brood sex ratio variance, developmentalmortality and virginity in a gregarious parasitoidwasp. Oecologia, 103: 162–69.
- Hardy, I.C.W. 2006. Bethylid wasps as model organismsfor studying contest behaviour. Paper presentedon Contests in Economics and Biology at SocialScience Research Center, Berlin in collaborationwith the Free University of Berlin, July 21–22,2006. 5p.
- Hardy, I. C. W. and Blackburn, T. M. 1991. Brood guardingin a bethylid wasp. Ecological Entomology,16: 55–62.
- Heimpel, G. E. 2000. Effects of the parasitoid clutch sizeon host-parasitoid population dynamics. In:Hochberg, M.E., Ives, A.R. (eds.), ParasitoidPopulation Biology. Princeton University Press,Princeton, pp. 27–40.
- Humphries, E. L., Hebblethwaite, A. J., Batchelor, T. P. and Hardy, I. C. W. 2006. The importance ofvaluing resources: host weight and contenderage as determinants of parasitoid wasp contestoutcomes. Animal Behaviour, 72: 891–898.
- Ichikawa, N. 1988. Male brooding behaviour of the giantwaterbug Lethocerus deyrollei Vuillefroy(Hemiptera: Belostomatidae). Journal ofEthology, 6: 121–127.
- Jalali, S. K., Rabindra, R. J., Rao, N. S. and Dasan, C. B.2003. Mass production of trichogrammatids andchrysopids. Project Directorate of BiologicalControl, Bangalore-560024, India. TechnicalBulletin No. 33: 16p.
- Kapadia, M. N. 1987. Occurrence and distribution ofdifferent parasitoids of Opisina arenosella Walkerunder Mahuva conditions of Gujarat. GujaratAgricultural University Research Journal,12: 17–21.
- Kishitani, Y. 1961. Observations on the egg-laying habit ofGoniozus japonicus Ashmead (Hymenoptera:Bethylidae). Kontyu, 29: 175–179.
- Luft, P. A. 1996. Fecundity, longevity and sex ratio ofGoniozus nigrifemur (Ashmead) (Hymenoptera:Bethylidae). Biological Control, 7: 17–23.
- Maynard-Smith, J. and Parkar, J. G. A. 1976. The logicof asymmetric contests. Animal Behaviour,24: 159–175.
- Morse, D. H. 1988. Interaction between the crab spiderMisumena vatia (Clerk) (Araneae) and itsichneumonid egg predator, Trychosis cyperiaTownes (Hymenoptera). Journal of Arachnology16: 132–135.
- Murdoch, W. W. and Briggs, C. J. 1996. Theory forbiological control: recent developments. Ecology,77: 2001–2013.
- Papaj, D. R. and Messing, R. H. 1998. Asymmetrics inphysiological state as a possible cause ofresident advantage in contests. Behaviour,135: 1013–1030.
- Payne, R. J. H. 1998. Gradually escalating fights andcumulative assessment model. AnimalBehaviour, 56: 651–662.
- Perez-Lachaud, G., Hardy, I. C. W. and Lachaud, J. P.2002. Insect gladiators: Competitive interactionbetween three species of bethylid wasps attackingthe coffee berry borer, Hypothenemus hampei (Coleoptera: Scolytidae). Biological Control,25: 231–238.
- Peterson, G. and Hardy, I. C. W. 1996. The importance ofbeing larger: parasitoid-intruder owner contestsand their implications for clutch size. AnimalBehaviour, 51: 1363–1373.
- Pillai, G. B. and Nair, K. R. 1985. Mating and hostparalyzing behaviour of Goniozus nephantidisMues. (Hymenoptera: Bethylidae) on Opisinaarenosella on coconut, pp. 123–125. Proceedingof National Seminar on Entomophagous Insects,Calicut, Kerala, India.
- Remadevi, O. K., Mohammed, U. V. K. and Abdurahiman,1981. Some aspects of the biology ofPerisierola nephantidis Muesebeck (Hymenoptera:Bethylidae) a larval parasitoid of Nephantisserinopa Meyrick (Lepidoptera: Xylorictidae). Polskie Pismo Entomologiczne, 51: 597–604.
- Stokkeb, S. and Hardy, I. C. W. 2000. The implication ofbeing gravid: egg laying and contest outcomein a parasitizing wasp. Animal Behaviour,59: 1111–1118.
- Tellamy, D. W. and Denno, R. F. 1986. Convergencepatterns in subsocial insects. Annual Review ofEntomology, 31: 369–390.
- Van Alphen, J. J. M. and Visser, M. E. 1990. Superparasitismas an adaptive strategy. Annual Review ofEntomology, 35: 59–79.
- Venkatesan, T., Jalali, S. K., Murthy, K. S. and Rao, N.S. 2003. Galleria mellonella (Linnaeus), analternate host for the rearing of Goniozusnephantidis (Muesebeck) (Hymenoptera:Bethylidae), a larval parasitoid of Opisinaarenosella Walker, pp. 79–82. In: Tandon,P. L., Ballal, C. R., Jalali, S. K. and Rabindra,R. J. (Eds.). Biological control of lepidopteranpests. PDBC, Bangalore 560024, India.
- Venkatesan, T., Jalali, S. K., Srinivasa Murthy, K., Rabindra,R. J. and Rao, N. S. 2004. Comparativelife table studies of Goniozus nephantidis(Muesebeck) (Hymenoptera: Bethylidae) onthree lepidopteran insect pests. Annals of PlantProtection Sciences, 12: 5–8.
- Venkatesan, T., Jalali, S. K., Srinivasa Murthy, K., Rabindra,R. J. and Rao, N. S. 2006. Field evaluationof different doses of Goniozus nephantidis(Muesebeck) for the suppression of Opisinaarenosella Walker on coconut. InternationalJournal of Coconut R&D (CORD), 22 (specialissue): 78–84.
- Venkatesan, T., Jalali, S. K. and Murthy, K. S. 2009. Competitive interactions between Goniozusnephantidis and Bracon brevicornis, parasitoidsof coconut pest Opisina arenosella. InternationalJournal of Pest Management, 55: 257–263.
- Venkatraman, T. V. and Chacko, M. J. 1961. Some factorsinfluencing the efficiency of Goniozus marasmiKurian, a parasite of maize and jowar leaf roller. Proceedings of the Indian Academy Sciences,53: 275–283.
- Genetic Variation in Artificially Selected Strains of the Egg Parasitoid, Trichogramma chilonis Ishii (Hymenoptera: Trichogrammatidae) Using Rapd Analysis
Authors
1 National Bureau of Agriculturally Important Insects, Post Bag No. 2491, H. A. Farm Post, Bellary Road, Bangalore 560024, Karnataka, IN
Source
Journal of Biological Control, Vol 23, No 4 (2009), Pagination: 353-359Abstract
Artificial selection is extensively used to develop pesticide resistance in natural enemies. RAPD markers were used to estimate genetic relatedness between the parent and artificially selected hybrids of the egg parasitoid Trichogramma chilonis Ishii resistant to multiple insecticides (700ppm of endosulfan, 540ppm of monocrotophos and 20ppm of fenvalerate) and high temperature (> 40°C). Highly polymorphic markers could be identified through the primers OPF-1 and OPJ-20. RAPD marker from 15 oligomers clearly outgrouped the susceptible parent from artificially selected pesticide-resistant strains. The first group comprised the susceptible strain. The second group comprised the two subclusters, the first subcluster including the strain resistant to endosulfan and fenvalerate, multiple-insecticide resistant strain (MIRS) and high temperature resistant (HTR) strain while the second subcluster consisted of monocrotophos and HTR strains. The discriminating property of RAPD markers allowed differentiation of the resistant strain from the parental susceptible strain. Artificially selected resistant strains shared relatively high similarity (61-66%) with susceptible parent strain as per Jaccard's index.Keywords
Trichogramma chilonis, RAPD, Pesticide Resistance, High Temperature, Genetic Relatednes.References
- Aljanabi, S. M., Loicacano, M. S., Lourenco, R. T., Borges,M. and Tigano, M. S. 1998. RAPD analysisrevealing polymorphism in egg parasitoid ofsoybean stink bugs (Hemiptera: Pentatomidae). Anais da Sociedade Entomologica do Brasil,27: 413-420.
- Ashok Kumar, G., Jalali, S. K., Venkatesan, T., Nagesh,M. and Lalitha, Y. 2008. Genetic improvementof egg parasitoid Trichogramma chilonis Ishii forcombined tolerance to multiple insecticides andhigh temperature. Journal of Biological Control,22: 347-356.
- Buso, G. S. C., Rangel, P. H. and Ferrira, M. E. 1998. Analysis of genetic variability of South Americanwild rice populations (Oryza glumaepatula) with isozymes and RAPD markers. Molecular Ecology,7: 107–117.
- Cenis, J. L. 1993. Indentification of four major Meloidogynespp. by random amplified polymorphic DNA(RAPD-PCR). Phytopathology, 83: 76-78.
- Dawson, I. K., Chalmers, K. J., Waugh, R. and Powell, W. 1993. Detection and analysis of genetic variationin Hordeum spontaneum populations from Israelusing RAPD markers. Molecular Ecology, 2: 151–159.
- Edwards, O. R. and Hoy, M. A. 1995. Random amplifiedpolymorphic DNA markers to monitor laboratoryselected,pesticide resistant Trioxys pallidus(Hymenoptera: Aphidiidae) after release intothree California walnut orchards. EnvironmentalEntomology, 24: 487-496.
- Hoy, M. A. 1994. Insect Molecular Genetics: Anintroduction to principles and applications, 2ndedition. Academic Press.
- Hsiao, J. Y. and Lee, S. M. 1999. Genetic diversity andmicrogeographic differentiation of Yushan cane(Yushania niitakayamensis; Poaceae) in Taiwan. Molecular Ecology, 8: 263–270.
- Huff, D. R., Peakall, R. and Smouse, P. E. 1993. RAPDvariation within and among a natural populationof outcrossing buffalo grass [Buchloë dactyloides(Nutt.) Engelm.]. Theoretical and AppliedGenetics, 86: 927–934.
- Jalali, S.K., Rabindra, R.J., Rao, N.S. and Dasan, C.B. 2003. Mass production of trichogrammatids andchrysopids. Project Directorate of BiologicalControl, Bangalore 560024, Technical BulletinNo. 33, 16pp.
- Jalali, S. K., Singh, S. P., Venkatesan, T., Murthy, K. S.,and Lalitha, Y. 2006a. Development of endosulfantolerant strain of an egg parasitoid Trichogrammachilonis Ishii (Hymenoptera: Trichogrammatidae). Indian Journal of Experimental Biology, 44: 584-590.
- Jalali, S. K., Venkatesan, T., Murthy, K. S., Rabindra, R. J.,Lalitha, Y., Udikeri, S. S., Patil, B. V., Bheemanna,M., Sreenivas, A. G., Balagurunathan, R. andYadav, D. N. 2006b. Field efficacy of multipleinsecticide tolerant strain of Trichogrammachilonis against American bollworm, Helicoverpaarmigera on cotton. Indian Journal of PlantProtection, 34: 173-180.
- Laurent, V., Wajenberg, E., Morgan, B., Schiex, T., Gaspin,C. and Vanlerberghe-Massuti, L. 1998. A compositegenetic map of parasitoid wasp Trichogrammabrassicae based on RAPD markers. Genetics,50: 275-282.
- Kumar, L. S., Sawant, A. S., Gupta, V. S. and Ranjekar, P.K. 2001. Genetic variation in Indian populationsof Scirpophaga incertulas as revealed by RAPDPCRanalysis. Biochemical Genetics, 39: 43-57.
- Martin, C., Gonzalez-Bentio, M. E. and Iriondo, J. M. 1997. Genetic diversity within and among populationsof a threatened species: Erodium paularense Fern. Gonz & Izco. Molecular Ecology, 6: 813–820.
- Pornkulwat, S., Skoda, S. R., Thomas, G. D. and Foster,J. E. 1998. Random amplified polymorphic DNAused to identify genetic variation in ecotypes ofthe European corn borer (Lepidoptera: Pyralidae). Annals of the Entomological Society of America,91:719-725.
- Rohlf, F. 1998. NTSYS-pc. Numerical taxonomy andmultivariate analysis system (version 2.02j). Exeter Software Publishers.
- Shah, R., Armstrong, K., Worner, S. P. and Chapman, R. B. 2002. Investigation of a PCR-based methodfor insecticide resistance monitoring. PakistanJournal of Biological Sciences, 5: 1070-1073.
- Subramanian, S. and Mohankumar, S. 2006. Geneticvariability of the bollworm, Helicoverpaarmigera, occurring on different host plants. 8pp. Journal of Insect Science, 6: 26.
- Vanlerberghe-Masutti F. 1994. Detection of geneticvariability in Trichogramma populations usingmolecular markers. Norwegian Journal ofAgricultural Sciences, 16: 171-176.
- Whitten, M. J. and Hoy, M. A. 1999. Enhanced biologicalcontrol through pesticide selectivity, pp. 271–296. In: Fisher T., Bellows, T. S., Caltagirone, L. E.,Dahlsten, D. L., Huffaker, C. and Gordh, G. (Eds.). Handbook of Biological Control, Academic Press.
- Williams, C. L., Goldson, S. L., Baird, D. B. and Bullock,D. W. 1994. Geographical origin of an introducedinsect pest, Listronotus bonariensis (Kuschell), determined by RAPD analysis. Heredity,72: 412-419.
- Yli-Mattila, T., Paavanen-Huhtala, S., Fenton,B. and Tuovinen, T. 2000. Species andstrain identification of the predatory miteEuseius finlandicus by RAPD-PCR andITS Sequences. Experimental and AppliedAcarology, 24: 863-880.
- Zhao, G. F., Felber, F. and Kuepfer, P. 2000. Subpopulationdifferentiation of Anthoxanthum alpinum(Poaceae) along an altitudinal gradientdetected by random amplified polymorphicDNA. Acta Phytotaxonomica Sinica,38: 64–70.
- Biochemical and Molecular Diversity Analysis of Culturable Bacteria in Cotesia plutellae (Kurdjumov) (Hymenoptera: Braconidae), a Parasitoid of Diamondback Moth, Plutella xylostella (Linnaeus)
Authors
1 Division of Molecular Entomology, National Bureau of Agriculturally Important Insects, Post Bag No. 2491, H. A. Farm Post, Bellary Road, Hebbal, Bangalore 560 024, IN
Source
Journal of Biological Control, Vol 27, No 4 (2013), Pagination: 260–267Abstract
Geographical populations of Cotesia plutellae, a predominant endolarval parasitoid of the diamondback moth, Plutella xylostella (Linnaeus) were screened and analyzed for bacterial diversity. The culturable bacterial species were isolated and identified by sequence analysis of 16S rRNA gene. Eleven bacterial isolates were identified viz., Pseudomonas sp., Enterobacter cancerogenus, Bacillus spp., Pseudomonas putida, Pantoea agglomerans, Bacillus thuringiensis, Pantoea sp. and Bacillus cereus. The molecular characterization and phylogenetic analysis placed these phylotypes into two major classes i.e. Bacilli and Gamma proteobacteria. The evolutionary distance matrix (Pairwise distance) showed similarity between the sequences. The bacterial diversity observed was low in the different geographic populations. The nucleotide sequences were blasted and submitted to GenBank.Keywords
Bacteria, Cotesia plutellae, 16S rRNA, Symbiont.References
- Breznak JA, 1982. Intestinal microbiota of termites and other xylophagous insects. Ann Rev Microbiol. 36: 323–343.
- Campbell BC. 1990. On the role of microbial symbiontes in herbivorous insects. In: Bernays, E.A. (Ed.), Insect– Plant Interactions, Vol. 1. CRC Press, Boca Raton, 1–44.
- Chapman R.1990. The insect: Structure and function. Bristol, UK: Book Society and Hodder and Stoughton, Great Britain, 968 pp.
- Christopher AD, Francisco Perfectti, Jeremy DB, Laramy SE, John HW. 2010. The genetic basis of interspecies host preference differences in the model parasitoid Nasonia. Heredity (Edinb) 104 (3): 270–277.
- Consoli FL, Elliot WK. 2006. Symbiofauna associated with the reproductive system of Cotesia flavipes and Doryctobracon areolatus (Hymenoptera: Braconidae). Brazilian J Morphol Sci. 23: 463–470.
- David Bickford, David JL, Navjot SS, Peter KL. Ng, Rudolf M, Kevin W, Krista KI, Indraneil Das. 2006. Cryptic species as a window on diversity and conservation. Trends in Ecol Evol. 22(3): 148–155.
- Dhumale UM, Mangesh Pradip M, Basweshwar Someshwar G. 2009. Geographical variations and genetics of pyrethroid resistance in diamondback moth, Plutella xylostella L. Int J Integ Biol. 7(3): 175–180.
- Doughlas AE. 1994. Symbiotic Interactions: Oxford University Press, Oxford, 1994.
- Dillon RJ, Dillon VM. 2004. The gut bacteria of insects: non pathogenic interactions. Ann Rev Ent. 49: 71–92.
- Girin C, Bouletreau, 1995. Microorganisms associated variation in host infestation efficiency in a parasitoid wasp Trichogramma bourarachae (Hymenoptera: Trichogrammatidae). Experientia 51: 398–401.
- Iturbe OI, O’Neill SL. 2007. Wolbachia–host interactions: connecting phenotype to genotype. Curr Opi Microbiol. 10: 221–224.
- Kehinde O, Ademolu, Adewunmi B, Idowu. 2011. Occurrence and distribution of microflora in the gut regions of the variegated grasshopper Zonocerus variegatus (Orthoptera: Pyrgomorphidae) during Development. Zool Stud. 50: 409–415.
- Kranthi KR, Jadhav DR, Wanjari RR, Shakhir AS, Russel D. 2001. Carbamate and organophosphate resistance in cotton pests in India. Bull Ent Res. 91: 37–46.
- Madhusudan S, Jalali SK, Venkatesan T, Lalitha L, Prasanna Srinivas. 2011. 16s rRNA gene based identification of gut bacteria from laboratory and wild larvae of Helicoverpa armigera (Lepidoptera: Noctuidae) from tomato farm. The Bioscan. 6: 175–183.
- Madden TL, Tatusov RL, Zhang J. 1996. Application of network BLAST server. Meth Enzymol. 266: 131–141.
- Martin MM, Kuko JJ. 1984. Role of mycophargy and bacteriophargy in invertebrate nutrition. pp. 257–263. In: Anderson JM, Rayner DM, Walton D. (Eds.), Microbial Ecology. Cambridge, UK: Cambridge University Press.
- Mochiah MB, Ngi-Song AJ, Overholt WA, Stouthamer R. 2002. Wolbachia infection in Cotesia sesamiae (Hymeoptera: Braconidae) causes cyto-plasmic incompatability: implications for biological control. Biol Control 25: 74–80.
- Mandrioli M. 2009. The interaction insect-symbiont, rather than insect-pathogen, may open new perspectives in the understanding of the host choice in bacteria. Inv Surv J. 6: 98–101.
- Potting RPJ, Vet LEM, Overholt WA. 1997. Variation in host selection behaviour and reproductive success in the stem borer parasitoid, Cotesia flavipes (Hymenoptera : Braconidae), Bull Ent Res. 87: 515– 524.
- Rattan RS, Ashok BH, Annette Reinke, Gupta PR, Claus PWZ. 2011. Molecular evidence for the presence of endosymbiotic bacteria Wolbachia in Cotesia populations (Hymenoptera: Braconidae). J Asia –Paci Ent. 14: 183–185.
- Talekar, NS, Shelton, AM. 1993. Biology, ecology and management of the diamondback moth. Ann Rev Ent 38: 275–301.
- Tamura K, Nei M. 1993. Estimation of the number of nucleotide substitutions in the control region of mitochondrial DNA in humans and chimpanzees. Mol Bio Evol. 10: 512–526.
- Tamura K, Peterson D, Peterson, Stecher G, Neii M, Kumar S. 2011. MEGA5: Molecular evolutionary genetics analysis using maximum likelihood, evolutionary distance and maximum parsimony Methods. Mol Biol Evol. 28: 2731–2739.
- Thakur D, Bhuyan M, Majumdar S, Yadav, A, Hazarika LK, Harman N, Baruah AALH, Bora TC. 2005. Isolation, characterization, in-vitro antibiotic susceptibility and pesticide tolerance of gut bacteria from rice hispa, Dicladispa armigera (Olivier). Ind J Microbiol. 45: 217–221.
- Wigglesworth VB. 1929. Digestion in the tsetse-fly: a study of structure and function. Parasitology 21: 288–291.
- Neochrysocharis Nr. Diastatae (Howard) (Hymenoptera:Eulophidae) Parasitic on Eggs of Letana Walker (Orthoptera:Tettigoniidae) in India:First Record of Host Association
Authors
1 ICAR-National Bureau of Agricultural Insect Resources, Post Bag No. 2491, H. A. Farm Post, Bellary Road, Hebbal, Bengaluru 560 024, Karnataka, IN
2 Department of Entomology, University of Agricultural Sciences, GKVK, Bengaluru 560 065, IN
3 Natural History Museum (Entomology), Cromwell Road, London SW7 5BD, GB
Source
Journal of Biological Control, Vol 29, No 3 (2015), Pagination: 121-124Abstract
Species of Neochrysocharis Kurdjumov (Hymenoptera: Eulophidae) are potential biocontrol agents for many important agricultural pests. This paper reports, for the first time, gregarious parasitism of Neochrysocharis nr. diastatae (Howard) on eggs of Letana sp. (Orthoptera: Tettigoniidae) on the host plant Pterospermum reticulatum Wt.&Arn. (Malvaceae) in Karnataka, India. The eggs of Letana sp. were observed along the margin of the leaves of P. reticulatum, visually distinguished as oval shaped structures. This is the first record of a host-parasitoid association between a species of Neochrysocharis and eggs of a Tettigoniidae grasshopper. DNA analysis of the parasitoid confirms a 100% match with a record of an unidentified species of Neochrysocharis from Canada. The geographical distribution and host record indicates that there may be a "N. diastatae" complex that this species actually belongs to, rather than being N. diastatae itself as N. diastatae is a Nearctic species and mainly known from agromyzids.Keywords
Grasshopper, Gregarious Egg Parasitoid, Pterospermum reticulatum, Oriental Region.- Occurrence of Chrysoperla zastrowi arabica Henry et al. (Neuroptera: Chrysopidae), a Cryptic Song Species of Chrysoperla (Carnea-group), in India
Authors
1 Biological Control, Post Bag No. 2491, Bellary Road, Hebbal, Bangalore - 560024, Karnataka, IN
2 Biological Control, Post Bag No. 2491, Bellary Road, Hebbal, Bangalore - 560024, Karnataka., IN
Source
Journal of Biological Control, Vol 22, No 1 (2008), Pagination: 143-147Abstract
The Chrysoperla species (carnea-group) widely used in India in augmentative biological control programmes was found to be Chrysoperla zastrowi arabica Henry et al. The acoustic profile of the mating song of this species was analyzed and found to match that of C. zastrowi arabica, the song species characterized earlier as 'Cc5 generator'. The correct taxonomic name for this species remains to be determined as it is morphologically identical to C. sillemi (Esben-Petersen), a species already known from India. Molecular characterization of the species was also done and the DNA sequence of the ITS-2 region was deposited in GenBank (Accession No. DQ 825504, as that of C. sillemi). The implications of this finding are discussed.Keywords
Chrysopidae, Carnea-group, Chrysoperla zastrowi Arabica, C. sillemi, India, Molecular Characterization, Song Analysis.- Genetic Improvement of Egg Parasitoid Trichogramma chilonis Ishii for Combined Tolerance to Multiple Insecticides and High Temperature
Authors
1 Biological Control, Post Bag No. 2491, H. A. Farm Post, Bellary Road, Bangalore, 560024, Karnataka, IN
2 Biological Control, Post Bag No. 2491, H. A. Farm Post, Bellary Road, Bangalore, 560024, Karnataka, IN
3 Biological Control, Post Bag No. 2491, H. A. Farm Post, Bellary Road, Bangalore, 560024, Karnataka, IN
Source
Journal of Biological Control, Vol 22, No 2 (2008), Pagination: 347-356Abstract
A strain of Trichogramma chilonis Ishii, an effective parasitoid of lepidopteran pests was developed for tolerance to three major groups of insecticides, i. e., endosulfan (organochlorine), monocrotophos (organophosphate) and fenvalerate (synthetic pyrethroid) and to high temperature (32-38°C) through selection. After 81 generations of selection, there was an increase in parasitism from 35% to 90-95% and decrease in mortality from 100% to 57-70% after 6h of constant exposure to three insecticides and high temperature. Interestingly 46.8 and 2.9 fold increase in tolerance was observed in males compared to 18.5 and 1.3 fold increase in females of MITT (multiple-insecticide and temperature tolerant) strain when exposed to endosulfan and fenvalerate sprays, respectively, while in case of monocrotophos, females and males were 465-fold and 25-fold more tolerant, respectively, than susceptible strain. At higher temperatures of 40 and 45°C, the per cent mortality of tolerant adults was 0.0 and 9.2%, respectively, compared to 59.7 and 96.1% in susceptible population after 6h of exposure at these temperatures. At high variable temperature (32-38°C), per cent mortality in MITT was 57.1 compared to 98.5% in susceptible population after 24h of constant exposure. The mean per cent parasitism at 32°C, 36°C, 38°C and at variable temperature of 32-38°C was significantly higher in tolerant strain (46.7, 45.0, 18.3 and 63.3%) compared to susceptible strain (54.0, 6.7, 0.0 and 0.0%), respectively. These studies suggest that the improved strain of T. chilonis will provide effective control of the pest even at harsh climatic conditions and under high insecticide pressure in different economically important crops.Keywords
Egg Parasitoid, Genetic Improvement, High Temperature Tolerance, Multiple Insecticide Tolerance, Trichogramma chilonis.- Field Evaluation of Goniozus nephantidis (Muesebeck) against Coconut Black-Headed Caterpillar in Kerala Using Different Release Techniques
Authors
1 Biological Control of Crop Pests and Weeds College of Horticulture, Kerala Agricultural University, Vellanikkara, Thrissur, 680 656, Kerala, IN
2 Hebbal, P. B. No. 2491, Bellary Road, Bangalore 560 024, IN
Source
Journal of Biological Control, Vol 20, No 1 (2006), Pagination: 33-36Abstract
Many entomophagous insects attack the black-headed caterpillar of coconut, Opisina arenosella Walker during its developmental stages. Goniozus nephantidis (Muesebeck) is a gregarious larval parasitoid of O. arenosella. During summer months of 2003-04 and 2004-05 the parasitoid was evaluated in the field in Kerala by following two methods - trunk and crown release that were compared with control. There was significant reduction in the population of O. arenosella after third to sixth releases in treated palms, when compared to control palms. There was no significant difference between the two methods of release of G. nephantidis in reducing the population of O. arenosella. Hence farmers could easily and effectively adopt the trunk release method.Keywords
Eva Luation, Goniozus nephantidis, Methods of Release, Opisina arenosella.- Economics of Production of Goniozus nephantidis (Muesebeck), an Important Parasitoid of Coconut Black-Headed Caterpillar, Opisina arenosella (Walker) for Bio-Factories
Authors
1 Project Directorate of Biological Control, P. B. No. 2491, H.A. Farm Post, Bellary Road, Hebbal, Bangalore, 560 024, Karnataka, IN
Source
Journal of Biological Control, Vol 21, No 1 (2007), Pagination: 53-58Abstract
Black-headed caterpillar, Opisina arenosella (Walker), is a serious pest of coconut palms causing severe defoliation and yield loss. Goniozus nephantidis (Muesebeck), one of the dominant and effective parasitoids of O. arenosella, is being widely used in the biological control programme. Technology for the production and cost economies of G. nephantidis were worked out for the first time. The production of 3,25,000 parasitoids within a period of 6 months required charging of 225 wooden Corcyra boxes @ 75 nos./batch three times. Coreyra cephalonica (Stainton) was used as a laboratory host for rearing the parasitoid. Exposure of 2500 matured C. cephalonica larvae, was required in order to get I lakh parasitoids per month. The cost of production of 100,000 G. nephantidis cocoons was Rs. 27,600. The commercial cost of cocoon in India is Rs. 40,000 per 100,000 parasitoids and the profit would be Rs. 12,400 for producing 100,000 parasitoids. Benefit-Cost of the production of parasitoid was 1:1.45. Employment generated during the production process was four. Hence, this technology is highly feasible and can he adopted for the production and use against the pest. This mass production technology would be suitable for promoting localized production of G. nephantidis at village or district level especially for farmers, unemployed graduates, private and public sector units and NGOs.Keywords
Black-Headed Caterpillar, Coreyra cephalonica, Cost of Production, Fixed Cost, Goniozus nephantidis, Opisina arenosella, Variable Cost.- Preliminary Testing of some New Release Methods for Egg Parasitoid Trichogramma spp.
Authors
1 Project Directorate on Biological Control (ICAR), P. B . No. 2491, H. A. Farm Post, Bellary Road, Bangalore 560 024, Karnataka, IN
Source
Journal of Biological Control, Vol 19, No 2 (2005), Pagination: 99-103Abstract
Preliminary investigations were conducted in laboratory cages to test the efficiency of a novel release technique for egg parasitoid Trichogramma species and this was compared with the traditional techniques. The efficiency of the techniques was determined based on time taken for release, adult emergence and percentage egg parasitism. Mixing of eggs with carriers like talc (1:1 ratio) and agar solution (0.1%) recorded least time for application. Spraying of loose parasitised eggs mixed with agar solution was considered as the best treatment amongst the treatments where aqueous solutions were used as carriers. In treatments where loose parasitised eggs were mixed with various solid and aqueous carriers, per cent emergence was low ranging from 40.5 to 57.1% compared to 95.0 to 100.0% in release of adults, Tricho bit, Tricho capsules and loose eggs without any carrier. The lowest emergence was recorded when loose parasitised eggs were mixed with talc. Adult release, sprinkling of loose parasitised eggs mixed with vermiculite and semolina gave significantly higher parasitism compared to the other techniques of release. The results indicated that release of Trichogramma can also be tried by mixing with a spray solution (for eg. agar solution) with modification of sprayer nozzle or with solid carriers (for eg. vermiculite). Such techniques will be better understood by stakeholders and is expected to increase uptake of this important biological control agent.Keywords
Carriers, Emergence, Parasitism, Release Method, Trichogramma.- Development of Crocidolomia binotalis Zeller (Lepidoptera: Pyralidae) on a Semi Synthetic Diet
Authors
1 Project Directorate of Biological Control (ICAR), Post Bag No.2491, H. A. Farm Post, Bellary Road, Bangalore, 560 024, Karnataka, IN
Source
Journal of Biological Control, Vol 19, No 2 (2005), Pagination: 179-182Abstract
The mean developmental period of Crocidolomia binotalis Zeller was 32.5 days with a percentage larval survival of 65.1per cent and adult emergence of 56.6 per cent on a semi-synthetic diet, while these were 26.6 days, 79.1 and 83.2%, respectively when reared on cabbage leaves. The factors for the variations in the biological attributes when reared on the diets and the feasibility of utilizing semi-synthetic diet reared host for rearing the parasitoids are discussed.Keywords
Biological Parameters, Cabbage Leaf Webber, Crocidolomia binotalis, Semi-Synthetic Diet, Rearing.- A Novel Method of Field Release of Goniozus nephantidis (Muesebeck), an Important Primary Parasitoid of Opisina arenosella Walker on Coconut
Authors
1 Project Directorate of Biological Control (ICAR) Post Bag No. 2491, Bellary Road, Hebbal, Bangalore 560 024, Karnataka, IN
Source
Journal of Biological Control, Vol 17, No 1 (2003), Pagination: 79-80Abstract
Goniozus nephantidis (Muesebeck) is an important primary parasitoid of Opisina arenosella Walker in coconut eco-system. The method of release of G. nephantidis was standardized for the first time. It was found that 90-100 per cent of the parasitoids released at the trunk (1.2 m from the ground level) reached the crown of the palm irrespective of the height of the tree. The mean time taken by each batch of the parasitoids to reach the crown varied from 13 to 22 minutes. It was also found that the parasitoids preferred to crawl on the tree rather than flying. Hence it is suggested that G. nephantidis adults may be released at the trunk (1.2 m height from the ground level) of the coconut palm for the management of O. arenosella instead of releasing at the crown region of the palm or arbitrarily on unit area basis.Keywords
Goniozus nephantidis Method of Release, Opisina arenosella.- Parasitising Efficiency of the Pupal Parasitoid, Tetrastichus howardi (Olliff) (Hymenoptera: Eulophidae) on Chilo partellus (Swinhoe) at Different Exposure Periods
Authors
1 Division of Crop protection, Indian Institute of Sugarcane Research, Rae Bareli Road, Dilkusha, P.O., Lucknow 226 002, UP, IN
2 Project Directorate of Biological Control (ICAR), Post Bag NO.2491, H. A. Farm Post, Hebbal, Bellary Road, Bangalore 560 024, Karnataka, IN
Source
Journal of Biological Control, Vol 18, No 1 (2004), Pagination: 65-68Abstract
Pupae of Chilo partellus (Swinhoe) were exposed to one-day-old mated females of Tetrastichus howard(OlIifO) for different periods to determine optimum period of exposure for laboratory production. The percentage parasitism varied significantly from 20 to 80 with different exposure periods. The number of parasitoids obtained per pupa (138.0) and females (71 %) were significantly higher when pupae were exposure for 12 hours and it decreased significantly on increasing exposure period. Though the per cent parasitism was vlry low when the pupae were exposed for 12 hours, the number of parasitoids obtained/ 100 pupae was highest (2760). However, considering progeny production and per cent females obtained, 12 hours exposure period is most suitable for avoiding superparasitism in the lahoratory production of the parasitoid.Keywords
Chilo partellus, Exposure Period, Superparasitism, Tetrastichus howardi.- Development of Cryptolaemus montrouzieri Mulsant (Coleoptera: Coccinellidae), a Predator of Mealybugs on Freeze-Dried Artificial Diet
Authors
1 Project Directorate of Biological Control Post Bag No. 2491, H. A. Farm Post. Bellary Road Bangalore 560 024, Karnataka, IN
Source
Journal of Biological Control, Vol 15, No 2 (2001), Pagination: 139-142Abstract
Development of Cryptolaemus montrouzieri Mulsant (Coleoptera: Coccinellidae) was studied on a freeze-dried artificial diet devoid of insect components. The artificial diet was composed of beef liver (5 g), hen's egg yolk (5g), sucrose (1g), honey (1g), hydrolysed yeast (1g), milk powder (0.5g), brewer's yeast (0.5g), groundnut oil (0.3g), multivitamin (0.04g). vitamin E (0.04g), nipbagine (0.004g) and water (16 ml). Biological attributes of the artificial diet reared C. montrouzieri were compared with the mealybug, Maconellicoccus hirsutus (Green) reared. Mean adult emergence of the predators reared on artificial diet and mealybug reared were 58.0 and 90.0 per cent, respectively. Differences in developmental period, adult weight and female emergence between artificial diet and mealybug reared predators were non-significant. Pre-ovipositional period of the predators reared on artificial diet was significantly longer than the mealybug reared. The mean fecundity of artificial diet reared predator was only 8 eggs/female, which was significantly lower than the mealybug reared (204eggs/female). Artificial diet reared predators laid fertile eggs and the mean viability of the eggs was 93.0 per cent, which was not significantly different from the mealybug reared (94.0 %).Keywords
Artificial Diet, Biological Suppression, Cryptolaemus mantrouzieri, Maconellicoccus hirsutus, Planococcus citri- Host Range and Predatory Fauna of Aphis craccivora Koch (Homoptera:Aphididae) in Bangalore, Karnataka
Authors
1 Project Directorate of Biological Control, Post Bag No. 2491, H. A. Farm Post, Bellary Road, Bangalore 560 024, Karnataka, IN
Source
Journal of Biological Control, Vol 11, No 1&2 (1997), Pagination: 59-63Abstract
The aphid, Aphis craccivora Koch is a common pest of cowpea and lablab around Bangalore. Survey for its predatory fauna resulted in recording eleven coccinel1ids, six syrphids, a chamaemyiid and a hemerobiid species. Syrphid species viz., Betasyrphus fietcheri Ghorpade and B. linga Ghorpade are new records onA. craccivora in India and elsewhere. Among predators recorded, Cheilomenes sexmaculta (Fabricius), Paragus serratus (Fabricius) and Ischiodon scutellaris (Fabricius) were found predominant on A. craccivora.Keywords
Aphis craccivora, Cheilomenes sexmaculata, Predators, Syrphids.- Parasitising Ability of Some Trichogrammatid Species and Strains on Spodoptera exigua (Hubner)
Authors
1 Project Directorate of Biological Control, H.A.Farm post, P.B. No. 2491, Bangalore 560 024, IN
Source
Journal of Biological Control, Vol 10, No 1&2 (1996), Pagination: 117-119Abstract
Parasitising ability of some species and strains of trichogrammatids on Spodoptera exigua (Hubner) (Lepidoptera: Noctuidae) was studied in the laboratory. Trichogramma chilonis (cassia strain), T. chilonis Bio Sc 1 (sugarcane strain) and T. brasiliense parasitised more S. exigua eggs.
Keywords
Parasitisation, Spodoptera exigua, Strains, Trichogrammatids.Full Text
- Breeding of Campoletis chlorideae Uchida (Hymenoptera:Ichneumonidae) on Corcyra cephalonica Stainton
Authors
1 Project Directorate of Biological Control, Post Bag No. 2491, H. A. Farm Post, Hebbal, Bangalore-560 024, IN
Source
Journal of Biological Control, Vol 9, No 2 (1995), Pagination: 128-129Abstract
Campoletis chlorideae Uchida an early larval parasitoid of Helicoverpa armigera (Hiibner) was successfully reared on Corcyra cephalonica Stainton. The comparative biology of C. chlorideae was also studied on C. cephaionica, H. armigera and Spodoptera litura (Fabricius).Keywords
Biology, Campoletis chlorideae, Corcyra cephalonica, Rearing.- Potential Natural Enemies of the Invasive Rugose Spiraling Whitefly, Aleurodicus rugioperculatus Martin in India
Authors
1 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru - 560024, Karnataka, IN
2 Institute of Wood Science and Technology, Malleswaram, Bengaluru - 560003, Karnataka, IN
Source
Journal of Biological Control, Vol 30, No 4 (2016), Pagination: 236-239Abstract
A invasive rugose spiraling whitefly (RSW) Aleurodicus rugioperculatus Martin (Hemiptera: Aleyrodidae) was found infesting coconut, banana, custard apple and several ornamental plants in Tamil Nadu, Andhra Pradesh and Kerala for the first time in India. The identity of the pest species was determined through morphological and molecular tools. Furthermore cytochrome c oxidase-I gene (658 bp) of RSW was sequenced (GenBank accession number KY209909) which would serve as an ideal molecular diagnostic marker for its identification irrespective of its phenotypic plasticity. During the survey, several natural enemies were recorded and maximum parasitism was recorded by Encarsia guadeloupae Viggiani (Hymenoptera: Aphelinidae) and its COI gene was sequenced and deposited as Encarsia sp. (GenBank accession number KY223606). Per cent parasitism ranged from 20.0 to 60.0 % in different collection locations, highest parasitism being recorded in Kerala as compared to other states. The predators recorded were Mallada sp., few coccinellids and predatory mites. This communication is the first report of the rugose spiraling whitefly, its host plant range and associated natural enemies in India.Keywords
Aleurodicus Rugioperculatus, Host-Plants and Natural Enemies, Invasive Pest, Spiraling Whitefly.References
- Evans GA. 2008. The whiteflies (Hemiptera: Aleyrodidae) of the world and their host plants and natural enemies. Available from: http://keys.lucidcentral.org/keys/v3/ whitefly/ PDF_PwP% 20ETC/world-whitefly- catalog-Evans.pdf
- Dickey AM, Stocks IC, Smith T, Osborne L, McKenzie CL. 2015. DNA barcode development for three recent exotic whitefly (Hemiptera: Aleyrodidae) invaders in Florida. Florida Entomol. 98(2): 473–478.
- Francis AW, Stocks IC, Smith TR, Boughton AJ, Mannion CM, Osborne LS. 2016. Host plants and natural enemies of rugose spiraling whitefly (Hemiptera: Aleyrodidae) in Florida. Florida Entomol. 99(1): 150–153.
- Hayat M. 2011. Additions to the Indian Aphelinidae (Hymenoptera: Chalcidoidea) – III: The genus Encarsia Förster. Oriental Insects 45: 202–274.
- Hebert PDN, Penton EH, Burns JM, Janzen DH, Hallwachs W. 2004. Ten species in one: DNA barcoding reveals cryptic species in the neotropical skipper butterfly Astraptes fulgerator, PNAS. 101(41): 14812–14817.
- Kumar V, McKenzie CL, Mannion C, Stocks I, Smith T, Osborne LS. 2013. Rugose spiraling whitefly, Aleurodicus rugioperculatus Martin (Hemiptera: Aleyrodidae). EENY578. University of Florida, IFAS Extension. Available from: http://entnemdept.ufl.edu/ creatures/orn /Aleurodicus_rugioperculatus.htm
- Martin JH. 2004. The whiteflies of Belize (Hemiptera: Aleyrodidae) Part 1 - Introduction and account of the subfamily Aleurodicinae Quaintance and Baker. Zootaxa. 681: 1–119.
- Sundararaj R, Selvaraj K. Invasion of rugose spiraling whitefly, Aleurodicus rugioperculatus Martin (Hemiptera: Aleyrodidae): A potential threat to coconut in India. Phytoparasitica (In Press).
- Stocks I. 2012. Rugose spiraling whitefly host plants. Florida Department of Agriculture and Consumer Services (FDACS), Division of Plant Industry (DPI). Available from: http://monroe.ifas.ufl.edu/ pdf/Hort/ RSW_Host_ Plants_May _2012.pdf
- Stocks IC, Hodges G. 2012. The rugose spiraling whitefly, Aleurodicus rugioperculatus Martin, a new exotic whitefly in south Florida (Hemiptera: Aleyrodidae). Florida Department of Agriculture and Consumer Services, Division of Plant Industry. Available from: http://freshfromflorida.s3. amazonaws.com/ aleurodicusrugioperculatus-pest-alert.pdf
- Taravati S, Mannion C, Glenn H, Osborne L. 2013. Natural enemies of rugose spiraling whitefly, Aleurodicus rugioperculatus Martin (Insecta: Hemiptera: Aleyrodidae) in the south Florida landscape. ENY- 870. University of Florida, IFAS Extension. Available from: http://edis.ifas.ufl.edu/pdffiles/IN/IN100400. pdf
- Viggiani G. 1987. New species of Encarsia Förster (Hymenoptera: Aphelinidae), parasitoids of whiteflies. Bollettino del Laboratorio di Entomologia Agraria ‘Filippo Silvestri’. Portici. 44: 35–37.
- First Record of Invasive Rugose Spiraling Whitefly Aleurodicus rugioperculatus Martin (Hemiptera:Aleyrodidae) along with Parasitoids in Karnataka
Authors
1 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru - 560024, Karnataka, IN
2 Institute of Wood Science and Technology, Malleswaram, Bengaluru - 560003, Karnataka, IN
Source
Journal of Biological Control, Vol 31, No 2 (2017), Pagination: 74-78Abstract
Occurrence of the invasive rugose spiraling whitefly (RSW), Aleurodicus rugioperculatus Martin was found on coconut, banana, mango, guava, sapota, Indian almond, water apple, ball tree, rubber fig, butterfly palm, and ruffled fan palm for the first time in Karnataka. Severe damage was noticed in the coastal areas of Mangalore and Udupi and the infestation ranged from 20-35% in coconut and 24-38% in banana. Morphology and molecular based taxonomic tools were used to identity the pest and its natural enemies. Survey also revealed natural parasitism by the parasitoids Encarsia guadeloupae Viggiani and E. dispersa Polaszek (Hymenoptera: Aphelinidae) with 5-15% in coconut, 7-18% in banana and 22-30% in sapota. Besides, other commonly found natural enemies viz., Stethorus sp. associated with mites and Dichochrysa astur were also recorded. Furthermore, augmentation and conservation strategies for these parasitoids for the management of this invasive pest were discussed.Keywords
Aleurodicus rugioperculatus, Host-Plants, Invasive Pest, Natural Enemies, Rugose Spiraling Whitefly.References
- Dickey AM, Stocks IC, Smith T, Osborne L, McKenzie CL. 2015. DNA barcode development for three recent exotic whitefly (Hemiptera: Aleyrodidae) invaders in Florida. Florida Entomol. 98(2): 473–478. https://doi.org/10.1653/024.098.0213
- Dubey AK, David BV. 2012. Collection, preservation and preparation of specimens for taxonomic study of whiteflies (Hemiptera: Aleyrodidae). pp-01-19. In: David B.V. (Ed.). The whiteflies or mealywing bugs. LAP Lambert Academic Publisher, Germany.
- Evans GA. 2008. The whiteflies (Hemiptera: Aleyrodidae) of the world and their host plants and natural enemies, Available from: http://keys.lucidcentral.org/keys/v3/ whitefly/ PDF_PwP% 20ETC/ world-whitefly- catalogEvans. pdf (Accessed 6 March, 2017).
- Francis AW, Stocks IC, Smith TR, Boughton AJ, Mannion CM, Osborne LS. 2016. Host plants and natural enemies of rugose spiraling whitefly (Hemiptera: Aleyrodidae) in Florida. Florida Entomol. 99(1): 150–153. https://doi.org/10.1653/024.099.0134
- Kumar V, McKenzie CL, Mannion C, Stocks I, Smith T, Osborne LS. 2013. Rugose spiraling whitefly, Aleurodicus rugioperculatus Martin (Hemiptera: Aleyrodidae). EENY578. University of Florida, IFAS Extension, Available from: http://entnemdept.ufl.edu/creatures /orn/ Aleurodicus rugioperculatus.htm (Accessed 5 March 2017).
- Mandal FB. 2011. The management of alien species in India. Int J Biodivers Conser. 3(9): 467–473
- Martin JH. 1987. An identification guide to common whitefly pest species of the world (Homoptera: Aleyrodidae). J Trop Pest Manag. 33(4): 298–322. https://doi.org/10.1080/09670878709371174
- Martin JH. 2004. The whiteflies of Belize (Hemiptera: Aleyrodidae) Part 1 - introduction and account of the subfamily Aleurodicinae Quaintance & Baker. Zootaxa 681: 1–119.
- Ramani S, Poorani J, Bhumannavar BS. 2002. Spiraling whitefly, Aleurodicus dispersus Russell (Homoptera: Aleurodidae) in India. Biocontrol News and Information 23(2): 55–62.
- Selvaraj K, Sundararaj R, Venkatesan T, Chandish R. Ballal, Jalali SK, Ankita Gupta, Mrudula HK. 2016. Potential natural enemies of the invasive rugose spiraling whitefly, Aleurodicus rugioperculatus Martin in India. J Biol Control 30(4): 236-239.
- Stocks I. 2012. Rugose spiraling whitefly host plants. Florida Department of Agriculture and Consumer Services (FDACS), Division of Plant Industry (DPI), Available from: http://monroe.ifas.ufl. edu/ /Hort/ RSW _Host_ Plants_May _2012. pdf (Accessed 5 March 2017).
- Stocks IC, Hodges G. 2012. The rugose spiraling whitefly, Aleurodicus rugioperculatus Martin, a new exotic whitefly in south Florida (Hemiptera: Aleyrodidae).
- Florida Department of Agriculture and Consumer Services, Division of Plant Industry, Aleurodicus rugioperculatus, pest-alert.pdf (Accessed 7 March, 2017).
- Sundararaj R, Selvaraj K. 2017. Invasion of rugose spiraling whitefly, Aleurodicus rugioperculatus Martin (Hemiptera: Aleyrodidae): a potential threat to coconut in India. Phytoparasitica 45: 71-74, DOI:10.1007/ s12600-017-0567-0. https://doi.org/10.1007/s12600017-0567-0
- Taravati S, Mannion C, Glenn H, Osborne L. 2013. Natural enemies of rugose spiraling whitefly, Aleurodicus rugioperculatus Martin (Insecta: Hemiptera: Aleyrodidae) in the south Florida landscape. ENY-870. University of Florida, IFAS Extension, http://edis.ifas.ufl.edu/pdffiles/IN/IN100400.pdf. IN/IN100400.pdf (Accessed 4 March, 2017).
- Detection of Insecticide Resistance and Mechanisms of Resistance in Field Populations of Chrysoperla zastrowi Sillemi (Neuroptera:Chrysopidae) Collected from Different Geographical Locations in India
Authors
1 ICAR-National Bureau of Agricultural Insect Resources, P.B. No. 2491, H.A. Farm Post, Hebbal, Banaglore - 560024, Karnataka, IN
2 Regional Seri Cultural Research Station, Central Silk Board, Veeranam Road, Allikuttai Post, Vaikkalapattarai, Salem - 636003, Tamil Nadu, IN
Source
Journal of Biological Control, Vol 31, No 3 (2017), Pagination: 159-167Abstract
The toxic effect of commonly used insecticides in cotton fields was studied on 9 populations of Chrysoperla zastrowi sillemi (Esben-Petersen), an important predator of sucking pests collected in India. The dose mortality bioassay against 3-days old larvae was determined using three insecticides viz., endosulfan, fenvalerate and acephate by topical bioassay method. Mechanism of resistance to the above mentioned insecticides were determined without and with three metabolic inhibitors (synergists), viz., piperonyl butoxide (PBO), S,S,S-tributyl-phosphorotrithioate (DEF) and diethyl maleate (DEM). Among the populations, resistant ratios (RR) of CZS-8 was significantly higher i.e. 50.36., 66.11 and 277.51-fold for endosulfan, fenvalerate and acephate, respectively compared to susceptible population (CZS-10). The CZS-8 was selected for synergism study it showed higher LC50 values and resistance ratio for all three insecticides. It showed 8.97-fold, 18.49-fold and 6.38-fold increase in synergism ratio for endosulfan indicating the resistance was strongly synergised by PBO, DEF and DEM. Similarly for fenvalerate, CZS-8 showed 8.69-fold and 3.63-fold significant increase in synergism ratio by DEF and DEM, respectively and for acephate, CZS-8 showed 54.82-fold, 150.87-fold and 113.52-fold significant increase in synergism ratio indicating that the resistance could be due to cytochrome p-450, esterase and glutathione s- transferase activity. The study indicated that the field population of C. z. sillemi developed resistance to different groups of insecticides. Among different geographical populations, CZS-8 collected from Sriganganagar, was recorded as most resistant.Keywords
Chrysoperla zastrowi Sillemi, Cytochrome P450, Esterase, Glutathione–S-Transferase Insecticide Resistance.References
- Ahmad M, Hollingwoth R. 2004. Synergism of insecticides provides evidence of metabolic mechanisms of resistance in the obliquebanded leafroller Choritoneura rosaceana (Lepidoptera: Tortricidae). Pest MAnag Sci. 60: 465–473. Crossref PMid:15154513
- Armes NJ, Banerjee SK, DeSouza KR, Jadhav DR, King ABS, Kranthi KR, Regupathy A, Surulivelu T, Rao NV. 1994. Insecticide resistance in Helicoverpa armigera in India: recent developments. pp. 437–442. In Brighton Crop Protection Conference-Pests and Diseases-1994. The British Crop Protection Council. Farham, UK.
- Atkinson TH, Wadleigh RW, Koehler PG, Patterson RS. 1991. Pyrethroid resistance and synergism in a field strain of the German cockroach (Dictyoptera: Blattellidae). J Econ Entomol. 84: 1247–1250. Crossref PMid:1842795
- Bozsik A, Francis F, Gaspar C, Haubruge E. 2002. Effect of some insecticides on acetyl cholinesterase from beneficial insects: Coccinella septempunctata, Chrysoperla carnea and Forficula auricularia Mededelingen Faculteit Landbouwkundige en Toegepaste Biologische Wetenchappen, Universiteit Gent. 67: 671–677.
- Casida J. 1970. Mixed function oxidase involvement in the biochemistry of insecticide synergists J. Agric. Food Chem. 18: 753–772.
- Croft BA, Brown AWA. 1975. Responses of arthropod natural enemies to insecticides. Annu Rev Entomol. 10: 285–335. Crossref PMid:234711
- Croft BA, Briozzo J, Carbonell JW. 1976. Resistance to organophosphorous insecticides in a predaceous mite, Amblyseius chilenensis (Acarna: Phytoseidae). Econ Entomol. 69: 563– Crossref
- Dhawan AK, Singh S, Kumar S. 2009. Integrated Pest Management (IPM) helps to reduce pesticide load in cotton. J Agric Sci Tech. 11: 275–282
- Finney DJ. 1952. Probit Analysis. 2nd edition. Cambridge University. Press. 250 pp.
- Grafton-Cardwell EE, Hoy A. 1985. Intraspecific variability in response to pesticides in the common green lacewing, Chrysoperla carnea (Stephens) (Neuroptera: Chrysopidae). Hilgardia 53: 1–31. Crossref
- Gunning RV, Moores GD, Devonshire AL. 1998. Inhibition of resistance-related esterases by piperonyl butoxide in Helicoverpa armigera (Lepidoptera:Noctuidae) and Aphis gossypii (Hemiptera: Aphididae). pp. 215– 227 in: Jones, D.G. (Ed.) Piperonyl butoxide: The Insecticide Synergist, London, Academic Press.
- Gunning RV, Moores GD, Devonshire AL. 1999. Esterase inhibitors synergise the toxicity of pyrethroids in Australian Helicoverpa armigera (Hubner) (Lepidoptera: Noctuidae). Pestic Biochem Physiol. 63: 50–62. Crossref
- Henry CS, Brooks SJ, Johnson JB, Venkatesan T, Duelli P. 2010. The most important lacewing species in Indian agricultural crops, Chrysoperla sillemi (EsbenPetersen), is a subspecies of Chrysoperla zastrowi (Esben-Petersen) (Neuroptera: Chrysopidae). J Nat His. 44: 2543–2555. Crossref
- Kranthi KR, Jadhav DR, Wanjari R, Ali S, Russel DA. 2001. Carbamate and organophosphate resistance in cotton pests in India, 1995 to 1999. Bull Entomol Res. 91: 37–46. PMid:11228586
- Kranthi, KR, Jadhav DR, Kranthi S, Wanjari RR, Ali SS, Russell DA. 2002. Insecticide resistance in five major insect pests of cotton in India. Crop Prot. 21: 6: 449– 460. Crossref
- LI XC, Schuler MA, Berenbaum MR. 2007. Molecular mechanisms of metabolic resistance to synthetic and natural xenobiotics. Annu Rev Entomol. 52: 231–253. Crossref PMid:16925478
- Medina P, Budia PF, Del Estal P, Vi-uela V. 2003. Effect of three modern insecticides, pyriproxyfen, spinosad and tebufenozide, on survival and reproduction of Chrysoperla carnea adults. Ann Appl Biol. 142: 55. Crossref
- Motoyama N. 1980. Glutathione-S-transferases, their role in the metabolism of organophosphorous insecticides. Rev Biochem Toxicol. 2: 49–69.
- Narahashi T, Carter DB, Frey J, Ginsburg K, Hamilton BJ, Nagata K, Roy ML, Song J, Tatebayashi H. 1995. Sodium Channels and GABAA receptor-channel complex as targets of environmental toxicants. Toxicol Lett. 82/83: 239–245. Crossref
- Oppenoorth FJ. 1985. Biochemistry and genetics of insecticide resistance. pp. 731–773, In: Kerkut GA, Gilbert CI (Eds.). Comprehensive insect physiology, biochemistry and pharmacology, vol. 12. Pergamon, Oxford, UK.
- Pathan AK, Sayyed AH, Aslam M, Razaq, M, Jilani G, Saleem MA. 2008. Evidence of field-evolved resistance to organophosphates and pyrethroids in Chrysoperla carnea (Neuroptera: Chrysopidae). J Econ Entomol. 101: 1676–84. Crossref PMid:18950051
- Pathan AK, Sayyed, AH, Aslam M, Liu, TX, Razaq M, Gillani, WA. 2010. Resistance to pyrethroids and organophosphates increased fitness and predation potential of Chrysoperla carnea (Neuroptera: Chrysopidae). J Econ Entomol. 103: 823–834. Crossref PMid:20568629
- Picollo MI, Vassena CV, Mougabure C, Bernetti M, Zerba EN. 2000. Resistance to insecticides and effect of synergists on permethrin toxicity in Pediculus capitis (Anoplura: Pediculidae) from Buenos Aires. J Med Entomol. 37: 721–725. Crossref PMid:11004784
- Plapp FWJ, Bull DL. 1978. Toxicity and selectivity of some insecticides to Chrysoperla carnea, a predator of the tobacco budworm. Environ Entomol. 7: 431–434. Crossref
- Pree DJ, Archibald DE, Morrison RK. 1989. Resistance to insecticides in the common green lacewing Chrysoperla carnea (Neuroptera: Chrysopidae) in southern Ontorio. J Econ Entomol. 82: 29–54. Crossref
- Radika P, Subbaratnam GV. 2006. Insecticide resistance management in cotton- Indian Scenario. A review. Agric Rev. 27: 157–169.
- Reddy AS, Rao NV. 1989. Cotton whitefly review. Indian J Plant Prot. 17: 171–179.
- Robertson JL, Preisler HK. 1992. Pesticide Bioassays with Arthropods. 1st Edn., CRC Press, Boca Raton, Florida, ISBN-10: 0849364639, pp. 35–48.
- Scott JG. 1990. Investigating mechanisms of insecticide resistance methods, strategies and pitfalls. pp. 39–57 In: Roush RT, Tabashnik BE (Eds.). Pesticide resistance in Arthropods, New York, Chapman & Hall. Crossref PMid:10107655
- Sayyed AH, Pathan AK, Faheem U. 2010. Cross-resistance, genetics and stability of resistance to deltamethrin in a population of Chrysoperla carnea from Multan, Pakistan. Pestic Biochem Physiol. 98: 325–332. Crossref
- Symondron WUC, Sunderland KD, Greenstone MH. 2002. Can generalist predator be effective biocontrol agents? Ann Rev Entomol. 47: 561–594. Crossref PMid:11729085
- Valles SM, Koehler, PG, Brenner RJ. 1997. Antagonism of fipronil toxicity by piperonyl butoxide and S,S,Stributyl phophoro trithioate in the German cockroach (Dictyoptera: Blatellidae). J Econ Entomol. 90: 1254– 1258. Crossref
- Van Pottelberge S, Van Leeuwen T, Nauen R, Tirry L. 2009. Resistance mechanisms to mitochondrial electron transport inhibitors in a field collected strain of Tetranychus urticae Loch (Acari: Tetranychidae). Bull Ent Res. 99: 23–31. Crossref PMid:18590597
- Venkatesan T, Poorani, J, Jalali, S.K, Srinivasamurthy, K, Ashok Kumar, K, Lalitha Y, Rajeshwari R. 2008. Confirmation of the occurrence of Chrysoperla zastrowi arabica Henry et al. (Neuroptera: Chrysopidae) in India. J Biol Control 22: 143–147.
- Venkatesan T, Jalali, SK, Murthy KS, Rabindra RJ, Lalitha Y. 2009. Occurrence of insecticide resistance in field populations of Chrysoperla zastrowi arabica Henry et al. (Neuroptera: Chrysopidae) in India. Indian J Agric Sci. 79: 910–912.
- Wing KD, Schnee ME, Sacher M, Connair M. 1998. A novel oxadiazine insecticide is bioactivated in lepidopteran larvae. Arch Insect Biochem Physiol. 37: 91–103. Crossref
- Wu G, Jiang SB, Miyata T. 2004. Seasonal changes of methamidophos susceptible and biochemical properties in Plutella xylostella (Lepidoptera: Yponomeutidae) and its parasitoid Cotesisa plutellae (Hymenoptera: Braconidae). J Econ Entomol. 97: 1689–1698. Crossref PMid:15568361
- Wu G, Miyata T. 2005. Susceptibilities to methamidophos and enzymatic characteristics in 18 species of pest insects and their natural enemies to crucifer vegetable crops. Pestic Biochem Physiol. 82: 79–93. Crossref
- Yang RSH. 1976. Enzyme conjucation and insecticide metabolism. pp. 177–181. In: Wilkinson CF (Ed.). Biochemistry and Physiology of Insecticides. Plenum, New York. Crossref
- Young SJ, Gunning RV, Moores GD. 2005. The effect of piperonyl butoxide on pyrthroid-resistance-associated esterases in Helicoverpa armigera (Hubner) (Lepidoptera: Noctuidae). Pest Manag Sci. 61: 397– 401. Crossref PMid:15605351
- Zerba EN, De Licastro S, Wood E, Picollo MI. 1987. Insecticide mechanism of action, pp.103–106. In: Brenner R, Stoka A (Eds.) Chagas disease vectors. Vol. 3. CRC, Boca Raton, FL.
- Host-Insect and Host-Plant Associated Diversity in Microbiota Isolated from Most Important Oriental-Australian Region Egg Parasitoid
Authors
1 ICAR-National Bureau of Agricultural Insect Resources, Post Bag No. 2491, H. A. Farm Post, Bellary Road, Hebbal, Bangalore – 24, Karnataka, IN
2 ICAR-Indian Institute of Horticultural Research, Hessaraghatta Lake Post, Bangalore – 89, Karnataka, IN
Source
Journal of Biological Control, Vol 31, No 4 (2017), Pagination: 229-239Abstract
Host-insect and host-plant associated differentiation of genetically divergent microbiota were recorded from economically important egg parasitoid collected from 26 locations in India, Trichogramma chilonis constituted 86.8% of the populations collected. It was recorded from 14 host-insects, 14 different crops and weed plants from 12 states. Nine species of yeast were recorded from parasitoid from 5 host-insects with Wickerhamomyces anamalus was isolated from 36.4% samples and highest numbers were recorded from parasitoid collected on sugarcane. Bacillus cereus, Pseudomonas sp. and Stenotrophomonas maltophilia from T. chilonis constitute 64.3% of bacterial diversity based on their 16S rDNA sequences. For taxonomic identification using 16s rDNA and ITS sequences, we performed taxonomic classification of total 33 ITS isolates against UNITE Fungal ITS database and assigned taxonomy hierarchy to the sequences. Also, a total of 13 isolates 16s rDNA sequences were taxonomically assigned against RDP 16s rDNA database using RDP Naive Bayesian rRNA Classifier Version 2.1. Most of the species are correctly identified in the respective species members with high confidence threshold value support.Keywords
Egg Parasitoid, Evolutionary Relationship, Host-Insects, Host-Plants, Microbiota.References
- Bernays EA, Klein BA. 2002. Quantifying the symbiont contribution to essential amino acids in aphids: The importance of tryptophan for Uroleucon ambrosiae. Physiol Entomol. 27: 275–284. Crossref.
- Bignell DE. 1984. The arthropod gut as an environment for microorganisms. In: Anderson JM, Rayner ADAM, Walton Exeter DWH (eds.) Invertebrate-microbial interactions. Cambridge University Press, Cambridge, UK, pp. 205–227.
- Bilodeau E, Guay J-F, Turgeon J, Cloutier C. 2013. Survival to parasitoids in an insect hosting defensive symbionts: A multivariate approach to polymorphic traits affecting host use by its natural enemy. PLoS One. 8: e60708. Crossref. PMid:23565269 PMCid:PMC3614562
- Bourtzis K, Miller T. 2003. Insect symbiosis. CRC Press, Boca Raton, FL, USA, pp. 324. Crossref. PMCid:PMC1462605
- Broderick NA, Raffa KF, Handelsman J. 2006. Midgut bacteria required for Bacillus thuringiensis insecticidal activity. Proc Natl Acad Sci USA. 103: 15196-15199. Crossref. PMid:17005725 PMCid:PMC1622799
- Chandler JA, Morgan Lang J, Bhatnagar S, Eisen JA, Kopp A. 2011. Bacterial communities of diverse Drosophila species: Ecological context of a host-microbe model system. PLoS Genet. 7: e1002272. Crossref. PMid:21966276 PMCid:PMC3178584
- Colman DR, Toolson EC, Takacs-Vesbach CD. 2012. Do diet and taxonomy influence insect gut bacterial communities? Mol Ecol. 21: 5124–5137. Crossref. PMid:22978555
- de Souza DJ, Bézier A, Depoix D, Drezen JM, Lenoir A. 2009. Blochinannia endosymbionts improve colony growth and immune defence in the ant Camponotus fellah. BMC Microbiol. 9: 29. Crossref. PMid:19200360 PMCid:PMC2660346
- Deshpande V, Wang Q, Greefield P, Charleston M, PorrasAlfaro A, Kuske CR, Cole JR, Midgley DJ, Tran-Dinh N. 2016. Fungal identification using a Bayesian classifier and the ‘Warcup’ training set of internal transcribed spacer sequences. Mycologia 108: 1-5. Crossref. PMid:26553774
- Dillon RJ, Dillon VM. 2004. The gut bacteria of insects: Non pathogenic interactions. Annu Rev Entomol. 49: 71–92. Crossref. PMid:14651457
- Engel P, Martinsonb VG, Moran NA. 2012. Functional diversity within the simple gut microbiota of the honey bee. Proc Natl Acad Sci USA. 109: 11002–11007. Crossref. PMid:22711827 PMCid:PMC3390884
- Ferrari J, Godfray HC, Faulconbridge AS, Via S. 2006. Population differentiation and genetic variation in host choice among PEA aphids from eight host plant genera.
- Evolution. 60: 1574–1584. Crossref. PMid:17017058 Ferrari J, Scarborough CL, Godfray HCJ. 2007. Genetic variation in the effect of a facultative symbiont on host-plant use by pea aphids. Oecologia 153: 323–329. Crossref. PMid:17415589
- Ferrari J, Vavre F. 2011. Bacterial symbionts in insects or the story of communities affecting communities. Philos Trans R Soc Lond B Biol Sci. 366: 1389–1400. Crossref. PMid:21444313 PMCid:PMC3081568
- Gauthier J-P, Outreman Y, Mieuzet L, Simon J-C. 2015. Bacterial communities associated with host-adapted populations of pea aphids revealed by deep sequencing of 16S ribosomal DNA. PLoS One 10: e0120664.
- Crossref. PMid:25807173 PMCid:PMC4373712
- Hagen KS, Tassan RL, Sawall Jr EF. 1970. Some ecophysiological relationships between certain Chrysopa, honeydews and yeasts. Boll Lab Entomol Agrar Filippo Silvestri Portici. 28: 113–134.
- Hammer TJ, Dickerson JC, Fierer N. 2015. Evidence-based recommendations on storing and handling specimens for analyses of insect microbiota. Peer J. 18: 3e1190.
- Hansen AK, Moran NA. 2014. The impact of microbial symbionts on host plant utilization by herbivorous insects.
- Mol Ecol. 23: 1473–1496. Crossref. PMid:23952067 Hassan SA. 1997. Selection of species of Trichogramma for use in biological control programs. In: (Parra JRP, Zucchi RA (eds.) Trichogramma and Applied Biological Control, Piracicaba: ESALQ, Brazil, pp. 183–205. PMid:9272632
- Jalali SK, Singh SP. 1993. Superior strain selection of the egg parasitoid Trichogramma chilonis Ishii - Biological parameters. J Biol Control 7: 57-60.
- Jalali SK, Singh SP, Venkatesan T, Murthy KS, Lalitha Y. 2006. Development of endosulfan tolerant strain of an egg parasitoid Trichogramma chilonis Ishii (Hymenoptera: Trichogrammatidae). Indian J Exp Biol. 44: 584–590. PMid:16872050
- Kaufman MG, Klug MJ. 199.) The contribution of hindgut, bacteria to dietary carbohydrate utilization by crickets (Orthoptera: Gryllidae). Comp Biochem Physiol. 98: 117–123. Crossref.
- Lachance MA, Bowles JM. 2002. Metschnikowia arizonensis and Metschnikowia dekortorum, two new large-spore yeast species associated with floricolous beetles. FEMS Yeast Res. 2: 81–86. Crossref.
- Leonardo TE, Muiru GT. 2003. Facultative symbionts are associated with host plant specialization in pea aphid populations. Proc R Soc Lond B Biol Sci. 270: 209–212. Crossref. PMid:14667385 PMCid:PMC1809968
- McFall-Ngai MJ. 2007. Adaptive immunity: care for the community. Nature. 445: 153. Crossref. PMid:17215830
- Medina FF, Nachappa P, Tamborindeguy C. 2011. Differences in bacterial diversity of host-associated populations of Phyllexera notabilis Pergande (Hemiptrea: Phylloxeridae) in pecan and water hickory. J Evol Biol. 24: 761–771. Crossref. PMid:21261774
- Meyer JM, Hoy MA. 2008. Molecular survey of endosymbionts in Florida populations of Diaphorina citri (Hemiptera: Psyllidae) and its parasitoids Tamarixia radiata (Hymenoptera: Eulophidae) and Diaphorencyrtus aligarhensis (Hymenoptrea: Encyrtidae). Florida Entomol. 91: 294–304. Crossref.
- Montagna M, Chouaia B, Mazza G, Prosdocimi EM, Crotti E, Mereghetti V, Vacchini V, Giorgi A, Biase AD, Cervo R, Lozzia GC, Alma A, Bandi C, Daffonchio D. 2015. Effects of the diet on the microbiota of the red palm weevil (Coleoptera: Dryophthoridae). PLoS One. 10: e0117439. Crossref. PMid:25635833 PMCid:PMC4311986
- Mrazek J, Strosova L, Fliegerova K, Kott T, Kopency J. 2008. Diversity of insect intestinal microflora. Folia Microbiol. 53: 229–233. Crossref. PMid:18661298
- Nagarkatti S, Nagaraja H. 1978. Experimental comparison of laboratory reared vs. wild-type Trichogramma confusum (Hym.: Trichogrammatidae) I. Fertility, fecundity and longevity. BioControl. 23: 129–136.
- Ngo CT, Aujoulat F, Veas F, Jumas-Bilak E, Manguin S. 2015. Bacterial diversity associated with wild caught Anopheles mosquitoes from Dak Nong Province, Vietnam using culture and DNA Fingerprint. PLoS One. 10: e0118634. Crossref. PMid:25747513 PMCid:PMC4352016
- Nguyen NH, Suh SO, Erbil CK, Blackwell M. 2006. Metschnikowia noctiluminum sp. nov., Metschnikowia corniflorae sp. nov., and Candida chrysomelidae sp. nov., isolated from green lacewings and beetles. Mycol Res. 110: 346–356. Crossref. PMid:16483756 Oliver KM, Moran RL, Hunter MS. 2005. Variation in resistance to parasitism in aphids is due to symbionts not host genotype. Proc Natl Acad Sci USA. 102: 12795–12800. Crossref. PMid:16120675 PMCid:PMC1200300
- Priya NG, Ojha A, Kajla MK, Raj A, Raman R. 2012. Host plant induced variation in gut bacteria of Helicoverpa armigera. PLoS One 7, e30768. Crossref. PMid:22292034 PMCid:PMC3266921
- Rizzi A, Crotti E, Borruso L, Jucker C, Lupi D, Colombo M, Daffonchio D. 2013. Characterization of the bacterial community associated with larvae and adults of Anoplophora chinensis collected in Italy by culture and culture-independent methods. BioMed Res Int. 2013: 420287. Crossref. PMid:24069601 PMCid:PMC3771249
- Simon JC, Carré S, Boutin M, Prunier-Leterme N, SabaterMunoz, Latorre A, Bournoville R. 2003. Host Based divergence in populations of the pea aphid: insights from nuclear markers and the prevalence of facultative symbionts. Proc Biol Sci. 270: 1703-1712. Crossref. PMid:12964998 PMCid:PMC1691435
- Srinatha HS, Jalali SK, Sriram S, Chakravarthy AK. 2015. Isolation of microbes associated with field-collected populations of the egg parasitoid, Trichogramma chilonis capable of enhancing biotic fitness. Biocontrol Sci Technol. 25: 789–802. Crossref.
- Stireman JO, Nason JD, Heard SB. 2005. Host-associated genetic differentiation in phytophagous insects: General phenomenon or isolated exceptions? Evidence from a goldenrod insect community. Evolution. 59: 2573–2587. Crossref. PMid:16526505
- Suh SO, Gibson CM, Blackwell M. 2004. Metschnikowia chrysoperlae sp. nov., Candida picachoensis sp. nov. and Candida pimensis sp. nov., isolated from the green lacewings Chrysoperla comanche and Chrysoperla carnea (Neuroptera: Chrysopidae). Int J Syst Evol Microbiol. 54: 1883–1890. Crossref. PMid:15388758
- Tagami Y, Doi M, Sugiyama K, Tatara A, Saito T. 2006. Survey of leafminers and their parasitoids to find endosymbionts for improvement of biological control. Biol Control. 38: 210–216. Crossref.
- Toju H, Fukatsu T. 2011. Diversity and infection prevalence of endosymbionts in natural populations of the chestnut weevil: relevance of local climate and host plants. Mol Ecol. 20: 853-868. Crossref. PMid:21199036 Tsuchida T, Koga R, Fukatsu T. 2004. Host plant specialization governed by facultative symbiont. Science. 303: 1989. Crossref. PMid:15044797
- Vorwerk S, Martinez-Torres D, Forneck A. 2007. Pantoea agglomerans-associated bacteria in grape phylloxera (Daktulosphaira vitifoliae, Fitch). Agric Forest Entomol. 9: 57–64. Crossref.
- Wang Q, Garrity GM, Tiedje JM, Cole JR. 2007. Naïve Bayesian classifier for rapid assignment of rRNA sequences into the new bacterial taxonomy. Appl Environ Microbiol. 73: 5261–5267. Crossref. PMid:17586664 PMCid:PMC1950982
- White TJ, Bruns TD, Lee SB, Taylor JW. 1990. Amplification and direct sequencing of fungal ribosomal RNA genes for phylogenetics. In: Innis MA, Gelfand DH, Sninsky JJ, White TJ (Eds.) PCR Protocols: A guide to Methods and Applications. Academic Press: San Diego, U.S.A., 1990, pp. 315–322. Crossref.
- Yun JH, Roh SW, Whon TW, Jung M-J, Kim MS, Park D-S, Yoon C, Nam Y-D, Kim Y-J, Choi J-H, Kim J-Y, Shin N-R, Kim S-H, Lee W-J, Bae J-W. 2014. Insect gut bacterial diversity determined by environmental habitat, diet, developmental stage, and phylogeny of host. Appl Environ Microbiol. 80: 5254-5264. Crossref.
- Morphological and Molecular Characterization of Predatory Aquatic and Semi-Aquatic Bugs of India
Authors
1 Zoological Survey of India, M Block, New Alipore, Kolkata – 700053, West Bengal, IN
2 ICAR-National Bureau of Agricultural Insect Resources, H.A. Farm Post, Bellary road, Hebbal, Bangalore – 560024, Karnataka, IN
Source
Journal of Biological Control, Vol 32, No 2 (2018), Pagination: 75-80Abstract
In the present study, a total of eight species of aquatic and semi-aquatic Hemiptera collected from India were identified based on morphology and mitochondrial cytochrome oxidase gene I (COI). Details of morphology based identification and the utility of COI gene to identify the aquatic Hemiptera is discussed in this paper.Keywords
Aquatic and Semi-Aquatic Bugs, Cytochrome Oxidase I, Hemiptera, Taxonomy.References
- Hungerford HB, Matsuda, R. 1958. The TenagogonusLimnometra. Complex of the gerrinae. Kansas Univ Sci Bull. 39(9): 371–457.
- Jordon KHC. 1951. Zoogeographisce Betrachtungen uber das ostiliche Sachsen dargestelitandentschen Neuf under von Heteropteren. Zoologischer Anzeiger. 147: 79–84.
- Masters JC, Boniotto M, Crovella S, Roos C, Pozzi L, DelPero M. 2007. Phylogenetic relationships among the lorisoidea as indicated by craniodental morphology and mitochondrial sequence data. Am J Primatol. 69: 6–15. https://doi.org/10.1002/ajp.20322 PMid:17171677
- Mogi M. 2007. Insects and other invertebrate predators. In: Floore TG (ed). Biorational https://doi.org/10.2987/8756-971X(2007)23[93:IAOIP]2.0.CO;2.
- Nam VS, Yen NT, Holynska M, Reid JW, Kay BH. 2000. National progress in dengue control in Vietnam: survey for Mesocyclops (Copepoda), Micronecta (Corixidae), and fish as biological control agents. Am J Trop Med Hyg. 62: 5–10. https://doi.org/10.4269/ ajtmh.2000.62.5 PMid:10761718
- Ohba SY, Huynh TTT, Kawada H, Le LL, Ngoc HT. 2011. Heteropteran insects as mosquito predators in water jars in Southern Vietnam. J Vector Ecol. 36(1): 170–174. https://doi.org/10.1111/j.1948-7134.2011.00154.x PMid:21635655
- Thirumalai G. 1999. Aquatic and semi-aquatic Heteroptera (Insecta) of India. Ind Assoc Aquatic Biologists (IAAB). 7: 1–74.
- Thompson JD, Higgins DG, Gibson TJ, Clustal W. 1994. Improving the sensitivity of progressive multiple sequence alignment through sequence weighting, position-specific gap penalties and weight matrix choice. Nucleic Acids Res. 22(22):4673–80. https://doi.org/10.1093/nar/22.22.4673 PMid:7984417 PMCid: PMC308517
- Wang C, Zhou X, Li S, Schwinghammer M, Scharf ME, Buczkowski G, Bennett GW. 2009. Survey and identification of termites (Isoptera: Rhinotermitidae) in Indiana. Ann Entomol Soc Am. 102(6): 1029–1036. https://doi.org/10.1603/008.102.0611
- Studies on New Invasive Pest Spodoptera frugiperda (J. E. Smith) (Lepidoptera: Noctuidae) and its Natural Enemies
Authors
1 ICAR-National Bureau of Agricultural Insect Resources, H. A. Farm Post, Bellary Road, Hebbal, Bengaluru - 560024, Karnataka, IN
2 All India Coordinated Research Project on Small Millets, Univeristy of Agricultural Sciences, GKVK, Bengaluru - 560065, Karnataka, IN
Source
Journal of Biological Control, Vol 32, No 3 (2018), Pagination: 145-151Abstract
Occurrence of Spodoptera frugiperda (J. E. Smith) (Insecta: Lepidoptera: Noctuidae), commonly known as fall armyworm, in southern India is reported along with associated natural enemies. Severe damage was noticed in Chikkaballapur, Hassan, Shivamogga, Davanagere and Chitradurga during July-August 2018. The incidence ranged from 9.0 to 62.5 percent at various locations, maximum incidence was recorded in Hassan district followed by Chikkaballapur, Davanagere, Shivamogga and Chitradurga. Morphology and molecular based taxonomic tools were used for the identification of this pest. The GenBank accession number MH704433 of Chikkaballapur population was released on 1st August, 2018 and Barcode obtained from BOLD System-ID: AGIMP054-18. The survey also revealed natural parasitism by egg parasitoids viz., Telenomus sp. (Hymenoptera: Platygastridae) and Trichogramma sp. (Hymenoptera: Trichogrammatidae), gregarious larval parasitoid, Glyptapanteles creatonoti (Viereck) (Hymenoptera: Braconidae) solitary larval parasitoid, Campoletis chlorideae Uchida (Hymenoptera: Ichneumonidae), and a solitary indeterminate larval-pupal (Hymenoptera: Ichneumonidae: Ichneumoninae) parasitoid. Spodoptera frugiperda is the first host record for G. creatonoti across the globe. Glyptapanteles creatonoti, being a well established parasitoid of various noctuids in India and Malaysia, was capable of parasitizing S. frugiperda. Besides these, other commonly found bioagents viz., Forficula sp. (Dermaptera: Forficulidae) and entomopathogenic fungus Nomuraea rileyi (Farl.) Samson was also collected in large numbers. We report the natural enemy complex of S. frugiperda for the first time from India. The electro physiological response of Indian population of S. frugiperda male adults to pheromone was established. The studies to manage this pest by any/all means are in progress.Keywords
Karnataka, Maize, New Pest.References
- Benson DA, Karsch-Mizrachi I, Lipman DJ, Ostell J, Wheeler DL. 2005. Nucleic Acids Res. 33(Database issue): D34−8. https://doi.org/10.1093/nar/gki063 PMid:15608212 PMCid:PMC540017
- Folmer O, Black M, Hoeh W, Lutz R, Vrijenhoek R. 1994. DNA primers for amplification of mitochondrial cytochrome c oxidase subunit I from diverse metazoan invertebrates. Mol Mar Biol Biotechnol. 3: 294−299.
- PMid:7881515
- Ganiger PC, Yeshwanth HM, Muralimohan K, Vinay N, Kumar ARV, Chandrashekara K. 2018. First report on the occurrence of the fall armyworm, Spodoptera frugiperda (J. E. Smith) (Lepidoptera, Noctuidae), a New Pest in Karnataka, India. UAS, GKVK, Bengaluru.
- Goergen G, Kumar PL, Sankung SB, Togola A, TamòM. 2016. First report of outbreaks of the fall armyworm Spodoptera frugiperda (J E Smith) (Lepidoptera, Noctuidae), a new alien invasive Pest in West and Central Africa. PLoS ONE 11(10): e0165632. doi:10.1371/journal.pone.0165632. https:// doi.org/10.1371/journal.pone.0165632
- Hebert PDN, Cywinska A, Ball SL, deWaard JR. 2003. Biological identifications through DNA barcodes.
- Proc R Soc Lond B Biol Sci. 270: 313−321. https:// doi.org/10.1098/rspb.2002.2218 PMid:12614582 PMCid:PMC1691236
- ICAR-NBAIR. 2018. Pest alert: Spodoptera frugiperda (J. E. Smith) (Insecta: Lepidoptera). (published on 30/07/2018).
- IITA. 2018. Fall armyworm has reached the Indian subcontinent! Available from: http://www.iita.org/news-item/ fall-armyworm-has-reached-the-indian-subcontinent/ (published on 04/08/2018).
- Sharanabasappa, Swamy KCM. 2018. Presence of fall armyworm, Spodoptera frugiperda (J. E. Smith) (Lepidoptera: Noctuidae), an Invasive Pest on Maize in University jurisdiction. University of Agricultural and Horticultural Sciences, Shivamogga, Karnataka, India. Available from: https://drive.google.com/file/ d/1hEW58nhZViHPnRduCjRHVIfWhGASHLSH/viewwww.uahs.in (published on 20/07/2018).
- Steinmann H. 1993. Dermaptera. Eudermaptera II. Das Tierreich. 108: 1−711.
- Wilkinson DS. 1928. A revision of the Indo-Australian species of the genus Apanteles (Hym. Bracon.).
- Part II. Bull Entomol Res. 19: 109–146. http://dx.doi.org/10.1017/s0007485300020393
- New Record of Carinostigmus Tsuneki (Hymenoptera: Crabronidae: Pemphredoninae) Species in India and Identity of its Species using DNA Barcoding
Authors
1 Division of Genomic Resources, ICAR - National Bureau of Agricultural Insect Resources,Bangalore - 560024, Karnataka, IN
Source
Journal of Biological Control, Vol 33, No 1 (2019), Pagination: 70-75Abstract
Specimens of the aphid hunting wasp Carinostigmus Tsuneki (Hymenoptera: Crabronidae: Pemphredoninae) were collected from South India. Morphological identification revealed three species, and one of them, C. griphus Krombein, is new for India. Identification of the species is supported through COI partial gene-DNA Barcoding.Keywords
Carinostigmus, DNA Barcoding, Molecular Phylogeny, Sphecidae.References
- Aguiar A. P. 2012. A technique to dry mount Hymenoptera (Hexapoda) from alcohol in a few seconds, and its application to other insect orders. Zootaxa 3412: 53-61. https://doi.org/10.11646/zootaxa.3412.1.3
- Ball, S. L. & Armstrong,K. F. 2008. Rapid, One-Step DNA Extraction for Insect. J Econ Entomol. 101(2): 523-532. https://doi.org/10.1093/jee/101.2.523 PMid:18459420
- Bingham, C. T. 1890. The Fauna of British India Including Ceylon and Burma: Hymenoptera, I (Wasps and Bees) London, 583pp.
- Bohart, R. M. and Menke, A. S. 1976. Sphecid Wasps of the World: A Generic Revision. University of California Press, UAS, 695pp.
- Burdrys ER. 1987. Roiushchie osy rodov Stigmus Panzer and Carinostigmus Tsunemi (Hymenoptera, Sphecidae) dal’nego Vostoka SSSR. pp. 49-56. In: Lehr PA and Storoshev (Eds). Novye Dannye po Sistematike Nasekomykh Dal’nego Vostoka Biological Pedological Institute, Far East Section, Academy of Science.
- Green, E. E. 1903. On the nesting habits of Trypoxylon intrudens and Stigmus niger. Spolia Zeylan. 1: 68-70.
- Hebert, P. D. N., Penton, E. H., Burns, J. M., Janzen, D. H. & Hallwachs, W. 2004. Ten species in one: DNA Barcoding reveals cryptic species in the Neotropical Skipper Butterfly Astraptes fulgerator. Proc Natl Acad Sci USA 101(41): 14812-14817. https://doi.org/10.1073/ pnas.0406166101
- Iwata, K. 1964. Bionomics of non-social wasps in Thailand. Nature Life Southeast Asia 3: 323-383.
- Khol, F. F. 1885. ZurSynonymie der Hymenoptera aculeata. Entomol Nachr Ber. 11: 161-165. http://biodiversitylibrary.org/page/10435649
- Krombein, K.V. 1984. Biosystematic Studies of Ceylonese Wasps, XIV: A Revision of Carinostigmus Tsuneki (Hymenoptera: Sphecoidea: Pemphredonidae).Smithsonian Contributions to Zoology, 396, Smithsonian Institution Press, City of Washington, 38 pp. https://doi.org/10.5479/si.00810282.396
- Ma L., Chen X.X. and LI Q. 2012. The genus Carinostigmus Tsuneki (Hymenoptera: Crabronidae) with two newly recorded species from China. Entomotaxonomia 34: 475-481.
- Mandakini Singla, Neha Goyal, Sobti RC and Sharma VL. 2015. Estimating molecular phylogeny of some Indian termites combining partial COI sequences. J Entomol Zool Studies 3(6): 213-218.
- Tamura K. and Kumar S. 2002. Evolutionary distance estimation under heterogeneous substitution pattern among lineages. Mol Biol Evol. 19: 1727-1736. https://doi.org/10.1093/oxfordjournals.molbev.a003995 PMid:12270899
- Tamura K, Nei M and Kumar S. 2004. Prospects for inferring very large phylogenies by using the neighbor-joining method. Proc Natl Acad Sci USA 101: 11030-11035. https://doi.org/10.1073/pnas.0404206101
- Tamura K, Glen Stecher, Daniel Peterson, Alan Filipski and Sudhir Kumar. 2013. MEGA6: Molecular Evolutionary Genetics Analysis Version 6.0. Mol Biol Evol.. 30(12): 2725-2729. https://doi.org/10.1093/molbev/mst197 PMid:24132122 PMCid:PMC3840312
- Tsuneki K. 1954. The Genus Stigmus Panzer of Europe and Asia with Descriptions of Eight New Species (Hymenoptera: Sphecidae). Memoirs of the Faculty of Liberal Arts, Fukui University, Series II (Natural Science), 3: 1-38.
- Tsuneki K, Nozaka C, Tano T, Kurokawa H and Murota T. 1992. Studies on the Philippine Sphecoidea. Hymenoptera. III. Special Publications of the Japan Hymenopterists Association. 40:1-86.
- Turner R.E. 1917. On a collection of Sphecoidea sent by the Agricultural Research Institute, Pusa, Bihar. Memoirs of the Department of Agriculture in India, 173-205.
- Walker F. 1860. Characters of some apparently undescribed Ceylon insects. Ann Mag Nat Hist. (Third Series) 6: 357-360. https://doi.org/10.1080/00222936008697340
- First Report of Exorista xanthaspis (Wiedemann, 1830) (Diptera: Tachinidae), A Larval-Pupal Parasitoid on Invasive Pest, Spodoptera frugiperda (J. E. Smith) in Maize from India
Authors
1 ICAR–National Bureau of Agricultural Insect Resources, Post Bag No. 2491, H. A. Farm Post, Bellary Road, Hebbal, Bengaluru − 560 024, Karnataka, IN
Source
Journal of Biological Control, Vol 34, No 1 (2020), Pagination: 82-85Abstract
For the first time, the tachinid fly, Exorista xanthaspis (Wiedemann, 1830) (Diptera: Tachinidae), was found to parasitize the larvae of fall armyworm, Spodoptera frugiperda (J. E. Smith) (Lepidoptera: Noctuidae) collected from maize fields in Karnataka, India. The field survey conducted during 2018-19 revealed the occurrence of E. xanthaspis on the larvae of S. frugiperda with the parasitism rate of 1.85 to 4.55% in maize fields. The identity of tachinid parasitoid was confirmed by amplifying Cytochrome Oxidase I gene (CO1-658 bp) and DNA.
Keywords
Parasitoid, Spodoptera frugiperda, Tachinid Fly.References
- Ballal CR, Kumar P, Ramani S. 1995. Laboratory evaluation, storability and economics of an artificial diet for rearing Chilo partellus (Swinhoe) (Lepidoptera: Pyralidae). J Entomol Res. 19: 135-41.
- Bhatnagar VS, Lateef SS, Sithanantham S, Pawar CS, Reed W. 1982. Research on Heliothis at ICRISAT; Proc. Int. Workshop on Heliothis Management, ICRISAT, Patancheru, Andhra Pradesh; p 385-96.
- CABI. 2019. Exorista xanthaspis. In: Invasive Species Compendium. Wallingford, UK: CAB International. www.cabi.org/isc/datasheet/23770.
- Crosskey RW. 1984. Annotated keys to the genera of Tachinidae (Diptera) found in tropical and southern Africa. Ann Natal Mus. 26(1): 189-337.
- Efil L, Kara K. 2004. Tachinid Parasitoids (Diptera: Tachinidae) of Spodoptera exigua in cotton fields in Diyarbakw, Turkey. Phytoparasitica 32(4): 363-66. https://doi.org/10.1007/BF02979846.
- EPPO. 2015. PM 7/124 (1) Spodoptera littoralis, Spodoptera litura, Spodoptera frugiperda, Spodoptera eridania.EPPO Bull. 45: 410-44. https://doi.org/10.1111/ epp.12258.
- Grenier S. 1988. Applied biological control with tachinid flies (Diptera, Tachinidae): A review. Anz Schadlingskde Pflanzenschutz Umweltschutz 61: 49-56. https://doi.org/10.1007/BF01906254.
- Hebert PDN, Cywinska A, Ball SL, DeWaard JR. 2003. Biological identifications through DNA barcodes. Proc R Soc Lond B Biol Sci. 270: 313-21. https://doi.org/10.1098/rspb.2002.2218. PMid: 12614582, PMCid: PMC1691236.
- Inclán DJ, Cerretti P, Marini L. 2014. Interactive effects of area and connectivity on the diversity of tachinid parasitoids in highly fragmented landscapes. Landsc Ecol. 29(5): 879-89. https://doi.org/10.1007/s10980014-0024-0.
- Kara K, Tschorsnig HP. 2003. Host catalogue for the Turkish Tachinidae (Diptera). J Appl Entomol. 127: 465-76. https://doi.org/10.1046/j.0931-2048.2003.00786.x.
- O’Hara JE, Henderson SJ, Wood DM. 2019. Preliminary checklist of the Tachinidae of the world. Version 1.0. PDF document, p. 681. Accessed 24 December 2019. Available at: http://www.nadsdiptera.org/Tach/ WorldTachs/Checklist/Worldchecklist.html.
- Patel AJ, Talati GM. 1987. Biology of Helicoverpa armigera (Hb.) as a pest of sunflower. Gujarat Agric Univ Res J. 12(2): 54.
- Prasanna BM, Huesing JE, Eddy R, Peschke VM. 2018. Fall Armyworm in Africa: A Guide for Integrated Pest Management, First Edition. Mexico, CDMX: CIMMYT.
- Qiu-Lin W, Li-Mei H, Xiu-Jing S, Yu-Ying J, Jie L, Gao H, Kong-Ming W. 2019. Estimation of the potential infestation area of newly-invaded fall armyworm Spodoptera frugiperda in the Yangtze River valley of China. Insects 10(9): 298. https://doi.org/10.3390/insects10090298. PMid: 31540256, PMCid: PMC6780859.
- Ratnasingham, S., Hebert, PDN. 2007. "BOLD: The Barcode of Life Data System (http://www.barcodinglife.org)". Mol. Ecol. Notes 7 (3): 355–364.
- Sambrook JF, Russell DW. 2001. Molecular Cloning: A Laboratory Manual, 3rd Edn. Cold Spring Harbor Laboratory Press, Cold Spring Harbor, New York, USA.
- Sharanabasappa, Kalleshwaraswamy CM, Poorani J, Maruthi MS, Pavithra HB, Diraviam J. 2019. Natural enemies of Spodoptera frugiperda (J. E. Smith) (Lepidoptera: Noctuidae), a recent invasive pest on maize in South India. Fla Entomol. 102(3):619-23. https://doi.org/10.1653/024.102.0335.
- Shylesha AN, Jalali SK, Gupta A, Varshney R, Venkatesan T, Shetty P, Ojha R, Ganiger PC, Navik O, Subaharan K, Bakthavatsalam N, Ballal CR. 2018. Studies on new invasive pest Spodoptera frugiperda (J. E. Smith) (Lepidoptera: Noctuidae) and its natural enemies. J Biol Control 32(3): 1−7.
- Sisay B, Simiyu J, Malusi P, Likhayo P, Mendesil E, Elibariki N, Mulatu Wakgari M, Ayalew G, Tefera T. 2018. First report of the fall armyworm, Spodoptera frugiperda (Lepidoptera: Noctuidae), natural enemies from Africa. J Appl Entomol. 142: 800-04. https://doi.org/10.1111/jen.12534.
- Stireman JO, O’Hara JE, Wood DM. 2006. Tachinidae: Evolution, behavior and ecology. Annu Rev Entomol. 51(1): 525-55. https://doi.org/10.1146/annurev.ento.51.110104.151133. PMid: 16332222.
- Tschorsnig H-P. 2017. Preliminary host catalogue of Palaearctic Tachinidae (Diptera). Tschorsnig. p. 480. http://www.nadsdiptera.org/Tach/WorldTachs/CatPalHosts/Cat_Pal_ tach_hosts_Ver1.pdf.
- Veenakumari K, Ramani S, Rabindra RJ. 2008. Additions to the natural enemy complex of the red hairy caterpillar, Anlsacta albistriga (Walker) (Lepidoptera: Arctiidae). J. Biol Control 22(1): 203-04.
- Verma SK. 1983. Exorista xanthapis (Wiedemann) (Tachinidae: Diptera), a new record on Amsacta moorei Butler. Ann Arid Zone. 22: 41-42.
- Visalakshi M, Ashika TR, Venkatesan T, Ballal CR, Laxman K, Nagarjuna D, Chittibabu G, Venkatarao P, Jamuna P. 2019. Report of the invasive fall armyworm, Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae) and its natural enemies on maize and other crops from Andhra Pradesh, India. J Entomol Zool Stud. 7: 1348-52.
- Occurrence of Fall Armyworm, Spodoptera frugiperda (J. E. Smith) (Lepidoptera: Noctuidae), in Chittoor District of Andhra Pradesh, India with a Note on Rove Beetle as its Potential Natural Enemy
Authors
1 Department of Entomology, S.V. Agricultural College, Tirupati - 517 502, Andhra Pradesh, IN
2 Administrative Office, Acharya N. G. Ranga Agricultural University (ANGRAU), Lam, Guntur - 522 034, A. P., IN
3 ICAR-National Bureau of Agricultural Insect Resources (ICAR-NBAIR), H. A. Farm Post, Hebbal, Bellary Road, Bengaluru – 560 024, Karnataka, IN
4 Department of Plant Pathology, S.V. Agricultural College, Tirupati, A. P., IN
Source
Journal of Biological Control, Vol 34, No 1 (2020), Pagination: 86-89Abstract
The occurrence of fall armyworm, Spodoptera frugiperda (J. E. Smith) (Lepidoptera: Noctuidae) in maize fields of Tirupati region, Andhra Pradesh is herewith reported. Field surveys in maize fields revealed that the rove beetle, Paederus fuscipes Curtis (Coleoptera: Staphylinidae) was found predating the larvae of fall armyworm and this is the first report of P. fuscipes on fall armyworm from India. The species identity of both fall armyworm and the rove beetle was confirmed through molecular studies by amplifying cytochrome oxidase I gene (CO1) and DNA barcoding.
Keywords
Fall Armyworm, Invasive Pest, Maize, Paederus fuscipes, Predator.References
- Benson DA, Karsch Mizrachi I, Lipman DJ, Ostell J, Wheeler DL. 2005. GenBank, Nucleic Acids Res. 33 (Database issue): D34−8. https://doi.org/10.1093/nar/gki063 PMid: 15608212 PMCid:PMC540017
- Clark MS. 1993. Generalist predators in reduced-tillage corn: predation on armyworm, habitat preferences, and a method to estimate absolute densities. Doctoral dissertation. Virginia Polytechnic Institute and State University.
- Day R, Abrahams P, Bateman M, Beale T, Clottey V, Cock M, Colmenarez Y, Corniani N, Early R, Godwin J, Gomez J, Moreno PG, Murphy ST, OppongMensah B, Phiri N, Pratt C, Richards G, Silvestri S, Witt A. 2017. Fall armyworm: impacts and implications for Africa. Outlooks Pest Manag. 28:196–201. https://doi.org/10.1564/v28
- Goergen G, Tam M. 2016. First report of outbreaks of the fall armyworm Spodoptera frugiperda (J E Smith) (Lepidoptera, Noctuidae), a new alien invasive pest in West and Central Africa. PLoS One 11: 1–5. https://doi.org/10.1371/journal.pone. 0165632.
- Hebert PDN, Cywinska A, Ball SL, deWaard JR. 2003. Biological identifications through DNA barcodes. Proc R Soc London, Series Bulletin. 270:313−321. https://doi.org/10.1098/rspb.2002.2218 PMid: 126145 82 PMCid:PMC1691236.
- Sharanabasappa D, Kalleshwaraswamy CM, Asokan R, Swamy HMM, Maruthi S, Pavithra HB, Hegde K, Navi S, Prabhu ST, Goergen G. 2018. First report of the fall armyworm, Spodoptera frugiperda (J. E. Smith) (Lepidoptera: Noctuidae), an alien invasive pest on maize in India. Pest Manag Hort Ecosyst. 24(1): 23–29
- Shylesha AN, Jalali SK, Gupta A, Varshney R, Venkatesan T, Shetty P, Rakshit Ojha R, Ganiger PC, Navik O, Subaharan K, Bakthavatsalam N, Ballal CR. 2018. Studies on new invasive pest Spodoptera frugiperda (J. E. Smith) (Lepidoptera: Noctuidae) and its natural enemies. J Biol Control. 32(3): 1–7 DOI: 10.18311/jbc/2018/21707.
- www.indiastat.com. 2016-17. State-wise area, production and productivity of tomato in India.
- Field evaluation of biopesticides against whitefly, Bemisia tabaci (Homoptera: Aleyrodidae) in tomato
Authors
1 Department of Agricultural Entomology, University of Agricultural and Horticultural Sciences, Shivamogga - 577204, Karnataka, IN
2 ICAR - National Bureau of Agricultural Insect Resources, Hebbal, Bellary Road Bengaluru - 560024, Karnataka, IN
Source
Journal of Biological Control, Vol 35, No 1 (2021), Pagination: 12-18Abstract
The efficacy of different biocontrol agents, botanicals and a biorational insecticide were evaluated against whitefly, Bemisia tabaci (Hemiptera: Aleyrodidae) in tomato under field conditions at Shivamogga, Karnataka during two seasons (Rabi 2018-2019 and summer 2019-2020). The results revealed that spiromesifen 240 SC @ 0.7 ml/L was the most effective in reducing the B. tabaci population i.e., 85.12 and 85.16 % reduction over untreated control during Rabi and summer, respectively followed by azadirachtin 5% @ 2 ml/l with reduction of 68.61 and 66.32 % over untreated control during Rabi and summer, respectively. The response of these treatments was also observed on the yield attributes, with highest fruit yield of 53.67 t/ha (6 pickings) in spiromesifen treatment followed by azadirachtin (52.93 t/ha), but the highest Benifit: Cost ratio was noticed in azadirachtin 5% (1:3.41), followed by spiromesifen 240 SC (1:3.38).Keywords
Azadirachtin, Bemisia tabaci, Bioagents, Biorational Insecticide, Botanicals, Tomato, Spiromesifen.References
- Abhijit G, Chatterjee ML and Anjan B. 2018. Field bioefficacy of some new insecticides and tank mixtures against whitefly on cotton in new alluvial zone of West Bengal. Pestic Res J. 30(1):1-7.
- Alam SKF, Patra B, Moulita C, Dey PK, Dhar PP, Samanta A and Somchoudhury AK. 2014. Bio efficacy of spiromesifen 240 Sc (w/v) against whitefly and red spider mites infesting tomato. J Entomol Res., 38(2): 01-10.
- Anonymous. 2015. NICRA team of Tomato Pest Surveillance 2012. Manual for Tomato Pest Surveillance. Jointly published by National Centre for Integrated Pest Management (NCIPM), New Delhi, Central Institute for Dryland Agriculture, Hyderabad, Indian Institute of Horticultural Research, Bengaluru and Indian Institute of Vegetable Research, Varanasi. 39p.
- Anonymous. 2018. Horticultural statistics at a glance.
- Asmita S and Ukey S P. 2014. Evaluation of certain botanicals, microbials: An conventional insecticide against mealybug infesting tomato. Int J Curr Microbiol Appl Sci. 3(11): 385-389.
- Basu AN. 1995. Bemisia tabaci (Gennadius): Crop pest and principal whitefly vector of plant viruses. Westview Press, New Delhi, 183p.
- Butani DK. 1977. Insect pest of vegetables-tomato. Pesticides, 11: 33-36.
- David BV, Ananthakrishnan TN. 2006. General and Applied Entomology. Second Edition. Tata McGraw-Hill Publishing Company Ltd. 27p.
- Legg JP. 1999. Emergence spread and strategies for controlling the pandemic of cassava mosaic virus disease in East and Central Africa. Crop Prot. 18: 627-637.
- Mahalakshmi MS, Sreekanth M, Adinarayana M and Rao YK. 2015. Efficacy of some novel insecticide molecules against incidence of whiteflies (Bemisia tabaci Genn.) and occurrence of Yellow Mosaic Virus (YMV) disease in urdbean. Int J Pure Appl Biosci. 3(5): 101-106.
- Nauen R, Bretschneider T, Bruck E, Elbert A, Reckmann U, Wachendorff U and Tiemann R. 2002. BSN 2060: A novel compound for whitefly and spider mite control. The BCPC Conference: Pests and Diseases, Vol. 1 and 2. Proceedings of the International Conference, Brighton, UK, 18-21 November, 2002. British Crop Protection Council, Farnham, UK, pp. 39-44.
- Noonari AM, Abro GH, Khuhro RD and Buriro AS. 2016. Efficacy of biopesticide for management of sucking insect pest of cotton, Gossypium hirsutum (L.). J Basic Appl Sci. 12: 306-313.
- Solangi BK, Suthar V, Riffat S, Abdul RAT, Muhammad N and Solangi MN. 2019. Screening of bio pesticides
- against insect pests of Tomato. Eur Acad Res. 5(2): 700-718.
- Sujay A, Anand B, Shankarganesh S and Karuppan. 2013. Efficacy of newer insecticides against leaf hopper and whitefly infesting brinjal and its effect on coccinellids. Indian Jf Plant Prot 25: 6-11.
- Tong XL. 2004. Toxicity and efficacy of spiromesifen, a tetronic acid insecticide, against sweet potato whitefly (Homoptera: Aleyrodidae) on melons and collards. Crop Prot. 23: 505-513.