Informatics Publishing Limited

Lalitha, Y.

• Intraguild Predation and Biosafety of Entomopathogenic Nematode, Heterorhabditis bacteriophora Poinar et Al., and its Bacterial Symbiont, Photorhabdus luminescens, to Parasitoid, Trichogramma chilonis Ishii and Predator Chrysoperla zastrowi sillemi (Esben, Petersen)

Abstract Views :321  |  PDF Views:129

Authors

Y. Lalitha ¹, M. Nagesh ¹, S. K. Jalali ¹

Affiliations
1 National Bureau of Agriculturally Important Insects, P.B. No. 2491, H.A. Farm Post, Hebbal, Bangalore 560 024, IN

Source

Journal of Biological Control, Vol 26, No 4 (2012), Pagination: 334–340

Abstract

Intraguild predation (IGP) appears to be pervasive among communities of biocontrol agents associated with nematode sharing the host with trophic interaction. Entomopathogenic nematode (Heterorhabditis bacteriophora) and its associated bacterium (Photorhabdus luminescens); an egg parasitiod, Trichogramma chilonis and a predator Chrysoperla zastrowi sillemi were selected for present study. There was no adverse effect of H. bacteriophora and P. luminescens observed on adult emergence of T. chilonis. Microscopic examination of eggs, larvae and adults of T. chilonis and C. z. sillemi treated with H. bacteriophora, P. luminescens and cell-free culture filtrates of P. luminescens, exhibited no deformity, discoloration or infection of organisms. Similarly, H. bacteriophora, P. luminescens or the cell-free culture filtrates exhibited no adverse activity on egg hatching or larvae of C. z. sillemi indicating that there was no intraguild competition under artificial epiphytotic conditions between the organisms under report, viz., H. bacteriophora, its associated bacterium (P. luminescens), T. chilonis and C. z. sillemi.

Keywords

Intraguild Predation, Entomopathogenic nematode, Heterorhabditis bacteriophora, Photorhabdus luminescens, Trichogramma chilonis, Chrysoperla zastrowi sillemi.

Full Text

   

References

• Akhurst RJ. 1980. Morphological and functional dimorphism in Xenorhabdus spp., bacteria symbiotically – associated with the insect pathogenic nematodes, Neoaplectana and Heterorhabditis. J Gene Microbiol. 121: 303–309.
• Boemare N, Laumond C Mauléon H. 1996. The entomopathogenic nematode-bacterium complex: Biology, life cycle and vertebrate safety. Bio Sci Tech. 6: 333–345.
• Ehlers RU. 1996. Current and future use of nematodes in biocontrol: Practice and commercial aspects with regard to regulatory policy issues Bio Sci Tech. 6: 303–316.
• Elzen GW, Elzen PJ, King EG. 1998. Laboratory toxicity of insecticide residues to Orius insidiosus, Geocoris punctipes, Hippodamia convergens and Chrysoperla carnea. Southwest Entomol. 23: 335–342.
• Fischer-Le Saux M, Viallard V, Brunel B, Normand P, Boemare N. 1999. Polyphasic classification of the genus Photorhabdus and proposal of new taxa. P. luminescens subsp. luminescens subsp nov., P. luminescens subsp. akhurstii subsp. nov., P. temperata subsp. temperata subsp. nov. and P. asymbiotica sp. nov. Int J Syst Bacteriol. 49: 1645–1656.
• Gaugler R, Wilson M, Shearer P. 1997. Field release and environmental fate of a transgenic entomo-pathogenic nematode. Biol. Control. 9: 75–80.
• Georgis R, Kaya HK, Gaugler R. 1991. Effect of steinernematid and heterorhabditid nematodes (Rhabditida: Steinernematidae and Heterorhabditidae) on nontarget arthropods Environ Entomol. 20: 815–822.
• Haag KH, Boucias DG. 1991. Infectivity of insect pathogens against Neochetina eichhorniae, a biological control agent of water hyacinth. Fla Entomol. 74: 128–133.
• Hassan SA. 1980. [A reproducible laboratory procedure for testing the persistence of the side-effect of pesticides on egg parasites of the genus Trichogramma (Hymenoptera: Trichogrammatidae.] Zeitschrift for Angewandie Entomologie 39: 282–289.
• Hassan SA. 1985. Standard methods to test the side-effects of pesticides on natural enemies of insects and mites developed by the IOBC/WPRS Working group Pesticides and beneficial organisms. Bulletin OEPP/ EPPO Bull. 15: 214–255.
• Jalali SK, Rabindra RJ, Rao NS, Dasan CB. 2003. Mass production of Trichogrammatids and chrysopids. Technical Bulletin No. 33, Project Directorate of Biological Control, H.A. Farm Post, Bellary Road, Hebbal, Bangalore 560 024, Karnataka, India, pp. 16.
• Jansson RK. 1993. Introduction of exotic entomopathogenic nematodes (Rhabditida: Heterorhabditidae and Steinernematidae) for biological control of insects: Potential and problems. Fla Entomol. 76: 82–96.
• Jaworska M, Ropek D, Prusznski S. 1995. The influence of entomopathogenic nematodes on insect natural enemies – Wplyw owadobojczych nicieni na wrogow naturalnych owadow Materialy Sesji Instytutu Ochrony Roslin. 35: 434–436.
• Kaya HK. 1978. Interaction between Neoaplectana carpocapsae (Nematoda: Steinernematidae) and Apanteles militaris (Hymenoptera: Braconidae), parasitoid of the armyworm, Pseudaletia unipuncta. J. Inv. Pathol. 31: 358–364.
• Kaya HK. 1984. Effect of the entomogenous nematode Neoaplectana carpocapsae on the tachinid parasite Compsilura concinnata (Diptera: Tachinidae). J Nematol. 16: 9–13.
• Li, Li-Yung. 1994. World-wide use of Trichogramma for biological control on different crops. A survey. In Biological Control with egg parasitoids (Eds: Wajnberg, E. and Hassan, SA). CAB International, Oxon, UK. Pp 37–53.
• Mohan S, Sabir N. 2005. Biosafety concern on the use of Photorhbdus luminescens as biopesticide: experimental evidence of mortality in egg parasitoid Trichogramma spp. Curr Sci. 89: 1268–1272.
• Mohan S, Raman R, Gaur HS. 2003. Foliar application of Photorahabdus luminiscens symbiotic bacteria from entomopathogenic nematode, Heterorhabditis indica to kill cabbage butter fly, Pieris brassicae. Curr. Sci. 84: 1397.
• Mohan S, Sirohi A, Gaur HS. 2004. Successful management of mango mealybug, Drosicha mangiferae by Photorhabdus luminescens, a symbiotic bacterium from entomopathogenic nematode Heteror-habditis indica. Int J Nematol. 14: 195–198.
• Mrácek Z, Spitzer K. 1983. Interaction of the predators and parasitoids of the sawfly, Cephalcia abietis (Pamphilidae: Hymenoptera) with its nematode Steinernema kraussei J Inv Pathol. 42: 397–399.
• Razek-Abdel AS. 2003. Pathogenic effects of Xenorhabdus nematophilus and Photorhabdus luminescens (Enterobacteriaceae) against pupae of the diamondback moth, Plutella xylostella (L.). J Pest Sci. 76: 108–111.
• Richardson PN. 1996. British and European legislation regulating rhabditid nematodes Bio Sci Tech. 6: 449–463.
• Rizvi SA, Hennessey R, Knott D. 1996. Legislation on the introduction of exotic nematodes in the US. Bio. Sci. Techo. 6: 477–480.
• Rosenheim JA, Kaya HK, Ehler LE, Marois JJ, Jaffee BA. 1995. Intraguild predation among biological-control agents: Theory and Evidence. Biol. Control. 5: 303–335.
• Smits PH. 1996. Post-application persistence of entomopathogenic nematodes. Bio Sci Tech. 6: 379–387.

• Influence of Seasons and Inoculum Dosages on the Production Efficiency of Corcyra cephalonica Stainton

Abstract Views :204  |  PDF Views:185

Authors

Y. Lalitha ¹, Chandish R. Ballal ¹

Affiliations
1 Division of Insect Ecology, National Bureau of Agriculturally Important Insects, Post Box No. 2491, H. A. Farm Post, Bellary Road, Bangalore, Karnataka, India Pin – 560024, IN

Source

Journal of Biological Control, Vol 29, No 1 (2015), Pagination: 25-30

Abstract

Corcyra cephalonica is a laboratory host used for multiplication of parasitoids, predators and entomopathogens. The present study is aimed to understand the effect of seasons and inoculum dosages of Corcyra eggs on the production efficiency. Egg production ranged from 3.1 to 5.8 cc per box during the different seasons and minimum production being recorded during dry months. The dosages tested were 0.5, 0.25 and 0.125 cc of Corcyra eggs / rearing box. Maximum per cent moth emergence (83.5%), shorter developmental duration (40.4 days) and higher fecundity (467 no.) of emerged moths were recorded in the boxes with 0.125 cc (2000 eggs) inoculum. Validation of experiments indicated that compared to the boxes with 0.5 cc inoculum, a 2.15, 1.44, 1.35 and 1.49 times increase in average production per box from 0.125cc infested boxes more during monsoon, post monsoon, dry and summer months, respectively. The data generated can be utilized for improving the protocol for mass rearing of Corcyra cephalonica.

Keywords

Corcyra cephalonica, Mass Production, Rearing Boxes.

Full Text

   

• Occurrence of Chrysoperla zastrowi arabica Henry et al. (Neuroptera: Chrysopidae), a Cryptic Song Species of Chrysoperla (Carnea-group), in India

Abstract Views :240  |  PDF Views:125

Authors

T. Venkatesan ¹, J. Poorani ², K. S. Murthy ¹, S. K. Jalali ¹, G. Ashok Kumar ¹, Y. Lalitha ¹, R. Rajeshwari ¹

Affiliations
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: 143-147

Abstract

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.

Full Text

   

• On the True Identity of "Trichogramma brasiliensis (Ashmead)" (Hyraenoptera: Trichogrammatidae) being Used in India

Abstract Views :254  |  PDF Views:109

Authors

H. Nagaraja ¹, Ankita Gupta ¹, Y. Lalitha ¹, P. Mohanraj ¹, S. K. Jalali ¹

Affiliations
1 Biological Control (ICAR), RB. No. 2491, H.A. Farm Post, Bellary Road, Hebbal, Bangalore, 560 024, Karnataka, IN

Source

Journal of Biological Control, Vol 22, No 2 (2008), Pagination: 255-260

Abstract

Investigations were carried out on the true identity of the thelytokous species purported to be Trichogramma brasiliensis (Ashmead) (= T. brasiliense), which is used in India in biological control programmes, as the holotype of Ashmead's species is placed under the genus Trichagratnmatoidea Girault at present. Morphological and molecular studies in combination with crossing experiments conclusively proved that this species was con specific with T. pretiosum Riley. Thelytoky in T. brasiliensis auctt. used in India is found to be Wolbachia - induced and reversible by administering antibiotics.

Keywords

Arrhenotoky, PCR, Ihelytoky, Trichogramma brasiliensis, Trichogramma pretiosum, Trichogrammatoidea, Wolbachia.

Full Text

   

• Genetic Improvement of Egg Parasitoid Trichogramma chilonis Ishii for Combined Tolerance to Multiple Insecticides and High Temperature

Abstract Views :221  |  PDF Views:110

Authors

G. Ashok Kumar ¹, S. K. Jalali ², T. Venkatesan ¹, M. Nagesh ², Y. Lalitha ³

Affiliations
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: 347-356

Abstract

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.

Full Text

   

• Preliminary Testing of some New Release Methods for Egg Parasitoid Trichogramma spp.

Abstract Views :232  |  PDF Views:146

Authors

S. K. Jalali ¹, K. S. Murthy ¹, T. Venkatesan ¹, Y. Lalitha ¹, P. S. Devi ¹

Affiliations
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: 99-103

Abstract

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.

Full Text

   

• Role of Egg Parasitoid, Trichogrammatoidea bactrae Nagaraja alone and in Combination with Dicblorovos in the Management of Plutella xylostella (Linnaeus) on Cabbage

Abstract Views :232  |  PDF Views:106

Authors

K. I. Singh ¹, S. K. Jalali ², R. J. Rabindra ², N. S. Rao ², Y. Lalitha ²

Affiliations
1 Department of Entomology, College of Agriculture, Central Agricultural University, lmphul 795 004, Manipur, IN
2 Project Directorate of Biological Control (lCAR), Post Bag no. 2491, Bellary Road, Hebbal, Bangalore 560 024, Karnataka, IN

Source

Journal of Biological Control, Vol 18, No 2 (2004), Pagination: 135-139

Abstract

The optimum release dosage of Trichogrammatoidea bactrae Nagaraja and its comparative efficacy alone and in combination with dichlorvos against diamondback moth (DBl\1), Plutella xylostella (Linnaeus) on cabbage was worked out. Results of the study on the percentage parasitization under different host-parasitoid ratios revealed that the maximum DBM egg parasitization (83.0%) was recorded in the ratio 100 (eggs): 5 (females), which was on par with other higher ratios of 100:10 to 100:20. The release of T. bactrae twice (2 and 5 days after DBM moth release) proved as the most effective treatment in significantly reducing the larval population (4.89 larvae per plant) in comparison to two sprays of dichlorvos (0.05%) (14.54 larvae per plant). The results indicated the efficacy of T. bactrae in suppressing DBM on cabbage and calls for further evaluation in field trials.

Keywords

Cabbage, Dichlorvos, Efficacy, Plutella xylostella, Trichogrammatoidea bactrae.

Full Text

   

• The New Invasive Pest Tuta absoluta (Meyrick) (lepidoptera: Gelechiidae) in India and its Natural Enemies along with Evaluation of Trichogrammatids for its Biological Control

Abstract Views :212  |  PDF Views:117

Authors

Chandish R. Ballal ¹, Ankita Gupta ¹, M. Mohan ¹, Y. Lalitha ¹, Abraham Verghese ¹

Affiliations
1 ICAR-National Bureau of Agricultural Insect Resources, Bellary Road, Bengaluru 560 024, IN

Source

Current Science, Vol 110, No 11 (2016), Pagination: 2155-2159

Abstract

The South American tomato moth Tuta absoluta (Meyrick) is a devastating pest of tomato. In the present study Tuta-adapted strains of Trichogramma were evaluated. Amongst the three species, Trichogramma achaeae Nagaraja and Nagarkatti, Trichogramma pretiosum Riley and Trichogrammatoidea bactrae Nagaraja could parasitise T. absoluta eggs and the parasitism rates were 5.0%, 51.1% and 68.2% respectively. Adults emerged from the parasitized T. absoluta eggs (4.8%, 97.5% and 90.0% adult emergence respectively). The F1 generation adults of T. pretiosum could parasitise 29% of Corcyra cephalonica Stainton eggs, while the other two species were not successful in parasitizing. In addition, four 'hymenopteran' parasitoids, viz. T. achaeae, Neochrysocharis formosa (Westwood), Habrobracon sp. and Goniozus sp. were also observed to be associated with T. absoluta in the fields during the surveys undertaken in southern India.

Keywords

Invasive Pest, India, Natural Enemies, Tuta absoluta.

Full Text

   

• 16S rRNA Gene Based Identification Of Gut Bacteria from Field Collected Larvae of Helicoverpa armigera (lepidoptera:Noctuidae) from Tomato Ecosystem

Abstract Views :388  |  PDF Views:0

Authors

S. Madhusudan ¹, S. K. Jalali ², T. Venkatesan ², Y. Lalitha ², Prasanna Srinivas ³

Affiliations
1 Department of Biotechnology, Maharani’s Science College for Women’s, Bengaluru, Karnataka, IN
2 Insect Biotechnology Laboratory, National Bureau of Agriculturally Important Insects (Formally PDBC), H.A. Farm Post, Hebbal, Bengaluru, Karnataka, IN
3 Department of Microbiology, Indian Academy Centre for Research and PG Studies, Hennur Cross, Bengaluru, Karnataka, IN

Source

Asian Journal of Bio Science, Vol 6, No 1 (2011), Pagination: 106-113

Abstract

Tomato fruit borer Helicoverpa armigera (Hübner) is a polyphagous pest of different host plants and has developed resistance to most of the insecticide groups. In order to know the gut microbial flora of the insecticide resistant field collected larvae of H. armigera, whole gut was dissected from the fourth to fifth instar larvae of the H. armigera and the culturable bacterial species were identified by sequence analysis of 16S rRNA gene. Altogether eleven bacterial species of different genera were identified were Stenotrophomonas sp., Enterococcus casseliflavus, Enterococcus sp., Enterococcus gallinarum, Enterococcus feacium, Bravundimonas diminuta, Staphylococcus sp., Pseudomonas aeruginosa, Acinetobacter calcoaceticus, Bacillus subtilis and Rhodococcus sp., of which genera Enterococcus were found to be predominant. The nucleotide sequences of 11 isolates were submitted to NCBI-Gen Bank and accession numbers (HM446252, HM446253, HM446254, HM446256, HM446258, HM446260, HM446261, HM446263, HM446264, HM446265, and HM446266) were obtained.

Keywords

Helicoverpa armigera, Gut Bacteria, 16S rRNA, Nucleotide, Sequencing.

Full Text

     

• Host-Insect and Host-Plant Associated Diversity in Microbiota Isolated from Most Important Oriental-Australian Region Egg Parasitoid

Abstract Views :246  |  PDF Views:132

Authors

S. K. Jalali ¹, S. Sriram ², T. Venkatesan ¹, R. P. More ¹, Omprakash Navik ¹, Y. Lalitha ¹, Rakshit Ojha ¹

Affiliations
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: 229-239

Abstract

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.

Full Text

   

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.

• Natural Parasitism by Trichogrammatids (Hymenoptera: Trichogrammatidae) on Lepidopteran Eggs under Diverse Cropping System

Abstract Views :248  |  PDF Views:117

Authors

Omprakash Navik ¹, S. K. Jalali ¹, Y. Lalitha ¹

Affiliations
1 Division of Germplasm Collection and Characterization, ICAR–National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru - 560024, Karnataka, IN

Source

Journal of Biological Control, Vol 33, No 3 (2019), Pagination: 279-284

Abstract

The present study was conducted to collect and identify the species of trichogrammatids from eggs of lepidopteran pests infesting the diverse cropping systems in the country. A total of 28 plant species were inspected for the collection of lepidopteran eggs either through collection of insect eggs or by placing sentinel egg cards. The species such as Trichogramma chilonis Ishii, T. achaeae Nagaraja and Nagarkatti, T. danausicida Nagaraja, Trichogrammatoidea bactrae Nagaraja and Tr. armigera Manjunath were recorded naturally occurring with 12 species of lepidopteran insect pests. In nature, the parasitism rate varied from 5.35 to 82.25% by the associated trichogrammatids. A total of 596 sentinel trap cards were placed in the agricultural, vegetables, fruits crops, and grasses on the bunds of fields to trap the egg parasitoids present in the different habitat. Through sentinel cards, three species, viz., T. chilonis, T. achaeae and Tr. bactrae were found inhabit the vegetables and ornamental crops. The percentage of adult emergence from the sentinel trap cards ranged from 70.59 to 100.0%. Natural parasitism of Tr. bactrae recorded for the first time on the eggs of Lampides boeticus L. infesting wild species of Crotalaria. In addition, the natural parasitism of Tr. armigera and Tr. bactrae on the eggs of L. boeticus laid on either cultivated or wild relatives of Crotalaria in undisturbed habitat had higher natural parasitism due to their bright yellow flower attracts parasitoids to parasitize the eggs and conserve these egg parasitoids. Recently, natural parasitism of Trichogramma sp. was recorded on invasive fall armyworm, Spodoptera frugiperda (J.E. Smith) infesting maize in Karnataka. Based on the present work, there could be choice of selecting right species which occur naturally on individual crops.

Keywords

Biological Control, Collection, Cropping System, Egg Parasitoid, Identification.

Full Text

   

References

• Alfred JRB, Das AK, Sanyol AK. 1998. Faunal Diversity in India. ENVIS Centre, Zoological Survey of India, Calcutta, 497 pp.
• Gardner J, Hoffmann MP, Pitcher SA, Happer JK. 2011. Integrating insecticides and Trichogramma ostriniae to control European corn borer in sweet corn: economic analysis. Biol Control 56: 9-16. https://doi.org/10.1016/j.biocontrol.2010.08.010
• Gurr GM, Wratten SD, Barbosa P. 2000. Success in conservation biological control of arthropods. P 105-132. In: G. Gurr and S. Wratten (Eds.), Biological control: Measures of success. https://doi.org/10.1007/978-94-011-4014-0_4
• Jalali SK, Omprakash Navik, Murthy KS, Venkatesan T, Lalitha Y. 2018. Predilection for host egg and host plant by trichogrammatid species collected from different Crops. Ann Pl Prot Sci 26(1): 1-5. https://doi.org/10.5958/0974-0163.2018.00001.0
• Jalali SK, Venkatesan T, Murthy KS, Rakshit Ojha. 2016. Management of Helicoverpa armigera (Hübner) on tomato using insecticide resistance egg parasitoid, Trichogramma chilonis Ishii in farmers’ field. Indian J Hortic 73(4): 611-614. https://doi.org/10.5958/0974-0112.2016.00123.7
• Macedo-Reis LE, Soares LGS, De Faria ML, Espírito-Santo MM, Zanuncio JC. 2013. Survival of a lepidopteran defoliator of Eucalyptus is influenced by local hillside and forest remnants in Brazil. Fla Entomol 96: 941-947. https://doi.org/10.1653/024.096.0331
• Manjunath TM, Phalak VR, Subramanian S. 1970. First records of egg-parasites of Heliothis armigera (Hubn.) (Lep.: Noctuidae) in India. Tech Bull Commonw Inst Biol Control 13: 111-115.
• Manjunath TM. 1972. Biological studies on Trichogrammatoidea armigera Nagaraja, a new dimorphic egg parasite of Heliorhis armigera (Hubner) in India. BioControl 17: 131-147. https://doi.org/10.1007/BF02371125
• Nagaraja H, Nagarkatti S. 1969. Three new species of Trichogramma (Hymenoptera: Trichogrammatidae) from India. BioControl 14(4): 393-400. https://doi.org/10.1007/BF02390544
• Nagaraja H. 1973. On some new species of Indian Trichogramma (Hymenoptera: Trichogrammatidae). Orient Insects 7(2): 275-290. https://doi.org/10.1080/0 0305316.1973.10434221
• Nagaraja H. 1978. Studies on Trichogrammatoidea (Hymenoptera: Trichogrammatidae). Orient Insects 12(4): 489-529. https://doi.org/10.1080/00305316.197 8.10432534
• Nagarkatti S, Nagaraja H. 1971. Redescriptions of some known species of Trichogramma (Hym., Trichogrammatidae), showing the importance of the male genitalia as a diagnostic character. Bull Entomol Res 61: 13-31. https://doi.org/10.1017/S0007485300057412
• Noyes JS. 1982. Collecting and preserving chalcid wasps (Hymenoptera: Chalcidoidea). J Nat Hist 16: 315-334. https://doi.org/10.1080/00222938200770261
• Querino RB, da Silva NNP, Zucchi RA. 2016. Natural parasitism by Trichogramma spp. in agroecosystems of the Mid-North Brazil. Cienc Rural 46: 1521-1523 https://doi.org/10.1590/0103-8478cr20151352
• Querino RB, Zucchi RA. 2003. Six new species of Trichogramma Westwood (Hymenoptera: Trichogrammatidae) from a Brazilian forest reserve. Zootaxa 134: 1-11 https://doi.org/10.11646/zootaxa.134.1.1
• Sivaraj N, Pandravada SR, Kamala V, Sunil N, Rameash K, Babu A, Elangovan M, Chakrabarty SK. 2016. Indian Crop Diversity. National Bureau of Plant Genetic Research. Retreived from: http://millets.res.in/books/chapter/Indian_crop_diversity.pdf https://doi.org/10.5958/0976-1926.2016.00004.8
• Souza RA, Giustolin TA, Querino RB, Alvarenga CD. 2016. Natural Parasitism of Lepidopteran Eggs by Trichogramma Species (Hymenoptera: Trichogrammatidae) in agricultural crops in Minas Gerais, Brazil. Fla Entomol 99(2): 221-225. https://doi.org/10.1653/024.099.0210
• Suroshe SS, Shankarganesh K, Paul B, Chandra Bose NS. 2015. Sentinel egg card studies for resident eggparasitoids harbouring horticultural crops of IARI, New Delhi campus. Indian J Hortic. 72(4): 578-580. https:// doi.org/10.5958/0974-0112.2015.00108.5
• Ulrichs CH, Mewis I. 2004. Evaluation of the efficacy of Trichogramma evanescens Westwood (Hymenoptera: Trichogrammatidae) inundative releases for the control of Maruca vitrata F. (Lepidoptera: Pyralidae). J Appl Entomol 128: 426-431. https://doi.org/10.1111/j.1439-0418.2004.00867.x
• Virgala MBR, Botto EN. 2010. Biological studies on Trichogrammatoidea bactrae Nagaraja (Hymenoptera: Trichogrammatidae), egg parasitoid of Tuta absoluta Meyrick (Lepidoptera: Gelechiidae). Neotrop Entomol. 39(4): 612-617. https://doi.org/10.1590/S1519-566X2010000400023

• Cross-resistance and biochemical mechanism in an insecticide-resistant population of Trichogramma chilonis Ishii (Hymenoptera: Trichogrammatidae) and its parasitizing efficiency against invasive fall armyworm Spodoptera frugiperda (J.E. Smith)

Abstract Views :129  |  PDF Views:80

Authors

Priyanka Dupatne ¹, T. Venkatesan ², Omprakash Navik ³, M. Mohan ³, K. M. Venugopal ³, Basavaarya ³, V. Linga ³, Y. Lalitha ³, G. Sivakumar ³, M. Ashwini ¹

Affiliations
1 Department of Entomology, University of Agricultural Sciences, Gandhi Krishi Vignan Kendra, Bellary Road, Bengaluru 560 065, India, IN
2 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, India, IN
3 ICAR-National Bureau of Agricultural Insect Resources, Hebbal, Bengaluru 560 024, India, IN

Source

Current Science, Vol 124, No 1 (2023), Pagination: 115-122

Abstract

Trichogramma chilonis is an egg parasitoid of lepidopteran pests and widely used in biological control and integrated pest management (IPM) programmes. In this study, the cross-resistance in multiple insecticide-tolerant strain of T. chilonis was evaluated against chlorantraniliprole 18.5% SC, spinetoram 11.7% SC and thiamethoxam 12.6% + lambda-cyhalothrin 9.5% ZC. Bioassay studies revealed the highest resistance level against chlorantraniliprole (8.83-fold resistance) over the susceptible population, followed by spinetoram (2.41-fold). Metabolic enzymes carboxylesterase and glutathione S-transferase showed major involvement in the resistant populations, with the highest activity obser­ved against chlorantraniliprole, followed by spinetoram. The resistant population at field recommended doses of chlorantraniliprole (400 ppm), parasitized 52.92% and 44.10% of Corcyra cephalonica and Spodoptera frugiperda eggs respectively, compared to 15.48% and 9.6% parasitism by the susceptible population. Integration and utilization of resistant strains of T. chilonis in IPM programmes can provide improved control of insect pests under insecticide-sprayed conditions and may reduce the insecticide load on crops

Full Text

   

References

• Zang, L.-S., Wang, S., Zhang, F. and Desneux, N., Biological control with Trichogramma in China: history, present status and perspec-tives. Annu. Rev. Entomol., 2020, 66(1), 463–484.
• Li, L.-Y., Worldwide use of Trichogramma for biological control on different crops: a survey. In Biological Control with Egg Para-sitoids (eds Wajnberg, E. and Hassan, S. A.), CAB International, Oxon, UK, 1994, pp. 37–53.
• Parra, J. R. P. and Coelho Jr, A., Insect rearing techniques for bio-logical control programs, a component of sustainable agriculture in Brazil. Insects, 2022, 13, 105.
• Khanh, D. T., Chailleux, H., Tiradon, A., Desneux, N., Colombel, E. and Tabone. E., Using new egg parasitoids (Trichogramma spp.) to improve integrated management against Tuta absoluta. EPPO Bull., 2012, 42, 249–254.
• Shylesha, A. N. et al., Studies on new invasive pest Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae) and its natural enemies. J. Biol. Control, 2018, 32, 145–151.
• Ganiger, P. C., Yeshwanth, H. M., Muralimohan, K., Vinay, N., Kumar, A. R. V. and Chandrashekara, K., Occurrence of the new invasive pest, fall armyworm, Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae), in the maize fields of Karnataka, India. Curr. Sci., 2018, 115(4), 621–623.
• Sharanabasappa, et al., First report of the fall armyworm, Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae), an alien invasive pest on maize in India. Pest Manage. Hortic. Ecosyst., 2018, 24, 23– 29.
• Sisay, B., Tefera, T., Wakgari, M., Ayalew, G. and Mendesil, E., The efficacy of selected synthetic insecticides and botanicals against fall armyworm, Spodoptera frugiperda, in maize. Insects. 2019, 10(2), 45.
• Navik, O., Shylesha, A. N., Patil, J., Venkatesan, T., Lalitha, Y. and Ashika, T. R., Damage, distribution and natural enemies of invasive fall armyworm Spodoptera frugiperda (J.E. Smith) under rainfed maize in Karnataka, India. Crop Prot., 2021, 143, 105536.
• Visalakshi, M. et al., Report of the invasive fall armyworm, Spodo-ptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae) and its natural enemies on maize and other crops from Andhra Pradesh, India. J. Entomol. Zool. Stud., 2019, 7(4), 1348–1352.
• Sharanabasappa, D., Pavithra, H. B., Kalleshwaraswamy, C. M., Shivanna, B. K., Maruthi, M. S. and Mota-Sanchez. D., Field efficacy of insecticides for management of invasive fall armyworm, Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae) on maize in India. Fla. Entomol., 2020, 103(2), 221–227.
• Venkatesan, T. and Jalali, S. K., Trichogrammatids: adaptation to stresses. In Biological Control of Insect Pests using Egg Parasitoids (eds Sithanantham, S. et al.). Springer India, New Delhi, 2013, pp. 105–125.
• Jalali, S. K., Venkatesan, T., Srinivasa Murthy, K. and Ojha, R., Management of Helicoverpa armigera (Hübner) on tomato using insecticide resistance egg parasitoid, Trichogramma chilonis Ishii in farmers’ field. Indian J. Hortic. 2016, 73(4), 611–614.
• Panini, M., Manicard, G. C., Moores, G. and Mazzoni, E., An overview of the main pathways of metabolic resistance in insects. Invertebr. Surviv. J., 2016, 13(1), 326–335.
• Ye, M. et al., The role of insect cytochrome P450s in mediating in-secticide resistance. Agriculture, 2022, 12, 53.
• Oakeshott, J. G., Claudianos, C., Campbell, P. M., Newcomb, R. D. and Russell, J. R., Biochemical genetics and genomics of insect esterases. In Comprehensive Molecular Insect Science (eds Gilbert, L. I., Iatro, K. and Gill, S.), Elsevier, The Netherlands, 2010, pp. 1–73.
• Kliot, A. and Ghanim, M., Fitness costs associated with insecticide resistance. Pest Manage. Sci., 2012, 68(11), 1431–1437.
• Nagaraja, H., Mass production of Trichogrammatid parasitoids. In Biological Control of Insect Pests using Egg Parasitoids (eds Sithanantham, S. et al.), Springer, New Delhi, 2013, pp. 175–189.
• Ballal, C. R., Kumar, P. and Ramani, S., Laboratory evaluation, storability and economics of an artificial diet for rearing Chilo par-tellus (Swinhoe) (Lepidoptera: Pyralidae). J. Entomol. Res., 1995, 19, 135–141.
• Kerima, O. Z., Niranjana, P., Lalitha, Y., Jalali, S. K. and Ballal, C. R., Inheritance of monocrotophos resistance in egg parasitoid Tricho-gramma chilonis (Ishii) (Hymenoptera: Trichogrammatidae). Curr. Agric. Res. J., 2017, 5(3), 297–304.
• Bradford, M. M., A rapid and sensitive method for the quantification of microgram quantities of protein utilizing the principle of protein-dye binding. Anal. Biochem., 1976, 74, 248–254.
• Van Asperen, K., A study of housefly esterases by means of a sen-sitive colorimetric method. J. Insect Physiol., 1962, 8, 401–416.
• Kinoshita, F. K., Frawley, J. P. and Du Bois, K. P., Quantitative measurement of induction of hepatic microsomal enzymes by various dietary levels of DDT and toxaphene in rats. Toxicol. Appl. Phar-macol., 1966, 9, 505–513.
• Saber, M., Acute and population level toxicity of imidacloprid and fenpyroximate on an important egg parasitoid, Trichogramma cacoeciae (Hymenoptera: Trichogrammatidae). Ecotoxicology, 2011, 20, 1476– 1484.
• Preetha, G., Stanley, J., Suresh, S. and Kuttalam, S., Toxicity of selected insecticides to Trichogramma chilonis: assessing their safety in the rice ecosystem. Phytoparasitica, 2009, 37(3), 208–215.
• Yang, Y., Wang, C., Xu, H., Tian, J. and Lu, Z., Response of Tricho-gramma spp. (Hymenoptera: Trichogrammatidae) to insecticides at concentrations sublethal to Cnaphalocrocis medinalis (Lepidoptera: Pyralidae). J. Econ. Entomol., 2020, 113(2), 646–653.
• Xie, L. C., Jin, L. H., Lu, Y. H., Xu, H. X., Zang, L. S., Tian, J. C. and Lu, Z. X., Resistance of lepidopteran egg parasitoids, Tricho-gramma japonicum and Trichogramma chilonis, to insecticides used for control of rice planthoppers. J. Econ. Entomol., 2022, 115(2), 446–454.
• Shankarganesh, K., Paul, B. and Gautam, R. D., Studies on ecological safety of insecticides to egg parasitoids Trichogramma chilonis Ishii and Trichogramma brasiliensis (Ashmead). Natl. Acad. Sci. Lett., 2013, 36(6), 581–585.
• Larson, J. L., Redmond, C. and Potter, D. A., Comparative impact of an anthranilic diamide and other insecticidal chemistries on benefi-cial invertebrates and ecosystem services in turfgrass. Pest Manage. Sci., 2011, 68(5), 740–748.
• Ashwini, M., Mohan, M., Sivakumar, G. and Venkatesan, T., Enhanced insecticide-resistance spectrum in green lacewing predator, Chrys-operla zastrowi sillemi (strain PTS-8) and its potential role in the management of sucking pests of cotton. Curr. Sci., 2021, 120(2), 423–428.
• Khan, M. A., Lethal and parasitism effects of selected novel pesticides on adult Trichogramma chilonis (Hymenoptera: Trichogrammatidae). J. Plant Dis. Prot., 2020,127, 81–90.
• Deshmukh, Y. V., Undirwade, D. B. and Dadmal, S. M., Effect of some newer insecticides on parasitization by Trichogramma species under laboratory condition. J. Entomol. Zool. Stud., 2018, 6(3), 228– 231.
• Khan, M. A., Khan, H. and Ruberson, J. R., Lethal and behavioral effects of selected novel pesticides on adults of Trichogramma pre-tiosum (Hymenoptera: Trichogrammatidae). Pest Manage. Sci., 2015, 71, 1640–1648.
• Zhang, J., Du, W., Jin, X., Ruan, C. and Zang, L., Susceptibility of the egg parasitoid Trichogramma dendrolimi (Hymenoptera: Trichogrammatidae) to three kinds of insecticides commonly used in fields. Acta Phytophyl. Sin., 2014, 41, 555–561.
• Costa, M. A., Moscardini, V. F., da Costa Gontijo, P., Carvalho, G. A., de Oliveira, R. L. and de Oliveira, H. N., Sublethal and trans-generational effects of insecticides in developing Trichogramma galloi (Hymenoptera: Trichogrammatidae): toxicity of insecticides to Trichogramma galloi. Ecotoxicology, 2014, 23(8), 1399–1408.
• Jalali, S. K., Singh, S. P., Venkatesan, T. and Murthy, K. S., Develop-ment of endosulfan tolerant strain of an egg parasitoid Tricho-gramma chilonis Ishii (Hymenoptera: Trichogrammatidae). Indian J. Exp. Biol., 2006, 44(2), 584–590.