Translator Disclaimer
1 September 2013 Baseline Susceptibility of Bemisia tabaci, Biotype B (Hemiptera: Aleyrodidae) to Chlorantraniliprole in Southern Florida
Rafael Caballero, Sabrina Cyman, David J. Schuster
Author Affiliations +
Abstract

Chlorantraniliprole 200 mg ai L-1 (Rynaxypyr® 200 SC) is the first xylem systemic insecticide in the new chemistry class, anthranilic diamides. A laboratory systemic bioassay using cut stems of cotton seedlings was developed to quantify the baseline susceptibility of the sweetpotato whitefly, Bemisia tabaci (Gennadius) biotype B, to chlorantraniliprole. Bioassays were conducted for a susceptible laboratory colony and for 11 field populations collected in 2008 and 2009 in Southern Florida. Baseline data of the susceptible colony (targeting first instar nymphs with initial exposure at the egg stage) for chlorantraniliprole in 2008 and 2009, revealed a pooled LC50 and slope values of 0.033 mg ai L-1 and 1.186, correspondingly. With the implementation of the stabilization period in the bioassay method in 2009, the susceptible colony generated LC50 and slope values of 0.182 mg ai L-1 and 0.972, respectively. LC50 and slope values of field collected populations (targeting nymphs as above) ranged from 0.016 to 0.046 mg ai L-1 and 0.889 to 1.595, respectively, in 2008 and 2009. Resistance ratio values at 50% mortality (RR50) on nymphs of field colonies ranged from 0.496 to 1.377. LC50 and slope values of the last 3 field collected populations of 2009, using the stabilization period, ranged from 0.117 to 0.251 mg ai L-1 and 0.885 to 1.395, respectively, and RR50 values ranging from 0.645 to 1.381. The overlapping of the fiducial limits of the LC50 values, the low RR50 values, and no significant differences in the slopes of the probit lines between the laboratory and field colonies, indicate that B. tabaci populations collected in Florida in 2008 and 2009 were highly susceptible to chlorantraniliprole. This anthranilic diamide insecticide is a promising tool in integrated pest management programs for B. tabaci, particularly where field populations have developed resistance to other insecticide groups. The baseline information developed in the present study confirmed the susceptibility of field populations in Florida and represents the basis for future susceptibility monitoring programs to help ensure the continued viability of chlorantraniliprole for B. tabaci management.

Since the introduction of the exotic biotype B of the sweetpotato whitefly [Bemisia tabaci (Gennadius)] in 1987 in Florida and the begomovirus Tomato Yellow Leaf Curl Virus (TYLCV) that it vectors in 1997, both have persisted as the major phytosanitary problem for tomato growers (Price 1987; Schuster et al. 1990; Kring et al. 1991; Brown et al. 1995; Polston et al. 1999). B. tabaci also reduces fruit quality and yield production by direct feeding on tomato leaves and also by inducing irregular riping of tomato fruits (Schuster et al. 1989, 1990). Florida is one of the main tomato growers, contributing to US tomato production with $ 620.2 and 564.7 million in 2010 and 2011, respectively, most of which consisted of fresh market tomatoes (USDA-NASS 2012). To keep this level of production, insecticides are used as the main mean for controlling the vector and reducing the virus incidence and severity in tomato crops. As a consequence, B. tabaci has developed resistance to all the insecticide chemistries used to control it (Cahill et al. 1996a, b, c; Palumbo et al. 2001; Toscano et al. 2001; Li et al. 2003; Horowitz et al. 2007). The discovery of new insecticidal compounds with unique modes of action and target sites is critical to the ongoing success of tomato crop protection.

Chlorantraniliprole (Rynaxypyr®, DPX-E2Y45, Coragen®, DuPont Crop Protection, Wilmington, Delaware) is a xylem systemic insecticide with a new mode of action in the new anthranilic diamide chemical class (DuPont 2008). The diamides belong to IRAC Group 28, the ryanodine receptor modulators (IRAC 2012). Insecticides in this class bind to and activate the ryanodine receptors in insect muscle cells, stimulating calcium release from the internal stores and causing impaired regulation, paralysis and death (Lahm et al. 2005, 2007 2009; Cordova et al. 2006, 2007; Legocki et al. 2008; Wilks et al. 2008). Chlorantraniliprole has demonstrated efficacy in the field against biotype B of B. tabaci, especially when applied to the root zone (Portillo et al. 2008; Schuster et al. 2008), and has been shown to be safe to non-target arthropods, including pollinators, numerous beneficial insects and predatory mites (Dinter et al. 2008; DuPont 2008; Preetha et al. 2009; Brugger et al. 2010; Shaw & Wallis 2010; Gradish et al. 2010, 2011).

Because of the potential for the development of resistance of B. tabaci to insecticides, a resistance management program was initiated in Florida in 2000 (Schuster & Thompson 2001). An integral part of that program included resistance monitoring of field populations, which initially focused on the neonicotinoid, imidacloprid, but was later expanded to include other neonicotinoids such as thiamethoxam, acetamiprid and dinotefuran; the pyrethroid bifenthrin; the organochlorine endosulfan; and the insect growth regulator buprofezin (Schuster & Thompson 2001, 2004; Schuster et al. 2002, 2003, 2006; Schuster 2007). As new products are developed for use in managing B. tabaci, it is necessary to develop a baseline susceptibility database prior to the registration and commercial use of the product that can be used as reference for future resistance monitoring efforts. Chlorantraniliprole (Rynaxypyr®) was registered as Coragen® in Florida in Aug 2008. Therefore, the objectives of the present investigation were to develop a bioassay in 2008 for estimating the susceptibility of B. tabaci to chlorantraniliprole and to use the bioassay to establish the baseline susceptibility of field-collected populations in Southern Florida. This method has since been published as the IRAC-approved method for testing chlorantraniliprole against B. tabaci.

MATERIALS AND METHODS

Host Plant

Cotton (Gossypium hirsutum L., var. ‘Deltapine 491’; Malvales: Malvaceae) was selected as the host plant to be used in the bioassays since it had been successfully used in previous systemic bioassays (Schuster et al. 2010; Caballero et al. 2013). Seedlings were grown inside organdycovered cages within an isolated greenhouse to ensure they were non-infested. Plants were used when the first true leaf had a diam of 2 cm.

Susceptible Whitefly Colony

A strain of biotype B of B. tabaci that had been maintained on tomato plants (Solanum lycopersicum L., var. ‘Lanai’; Solanales: Solanaceae) in the laboratory for almost 20 yr without exposure to insecticides and without reintroduction of whiteflies from the field was utilized for comparing the relative susceptibility of field populations to chlorantraniliprole. In this study, adults from the original susceptible colony were used to establish a new colony on cotton plants, since cotton was a more convenient host plant for the bioassays.

Field Populations

To establish field populations of B. tabaci, nymph-infested foliage was collected from commercial tomato fields in Southern Florida. Five populations were collected in the 2008 spring crop season, and 6 additional populations were collected during the spring of 2009. Collected foliage was placed in cages of 60 × 60 × 60 cm (BioQuip cat. 1450NS) with non-infested cotton plants maintained in a growth chamber at 26–28 °C with a photoperiod of 12:12 h L:D. The leaf samples were left in the cages for several days to allow as many adults as possible to emerge and settle. These emerged adults were considered the F1 generation. The whitefly populations were maintained on cotton plants for the duration of the testing. When insufficient adults in the F1 generation were available to conduct bioassays, the field populations were reared to the F2–F4 generations until sufficient adults were available.

Systemic Bioassay

The bioassay is a modification of the EARML method developed for the insect growth regulator buprofezin and was the same used to develop baseline susceptibility data for anthranilic diamides (Cahill et al. 1996c; Li et al. 2012; Caballero et al. 2013). Ten to 14 whitefly adults of unknown age and gender were aspirated and transferred to clip-cages (2 cm diam, 1 cm high) on the abaxial surface of the true leaf. Adults were allowed to lay eggs for 24 h then removed and the eggs were counted under a dissecting stereoscope. The sample size was uniformly adjusted to 25 eggs per leaf to avoid first instar competition and migration from leaves. In order to ensure homogeneous insecticide uptake, the height of the seedling stems was standardized to 15.25 cm from the terminal growth point by cutting each stem at its base. It was found that cutting the stems at a diagonal angle with a clean, disinfected scalpel on a cutting board significantly reduced problems with sudden death of seedlings during the bioassay due to contamination. For the last 3 field populations collected in 2009, as well as for the laboratory colony, a ‘stabilization period’ was included as an additional upgrade to the bioassay. This ‘stabilization period’ consisted of placing the cut stems in water for 24 h during the oviposition period prior to placing them in insecticide solution to ensure uniform saturation with water and, therefore, to ensure equal insecticide absorption. A dilution series of 4, 1, 0.25, 0.0625, 0.003906, and 0.000976 mg ai L-1 of chlorantraniliprole (Coragen® 200 SC, DuPont Crop Protection, Wilmington, Delaware) was prepared using double de-ionized water. An untreated control with water only was included. The cut stems were placed in the respective insecticide solutions in 13 mm diam × 60 mm long vials with a total volume of 8.5 cc (Fisher cat. 0333925C). The cut stems in vials were placed inside cages and these were maintained in a growth chamber at 26–28 °C at 12:12 h L:D for 14 days for hatching of eggs and for full development of second instar nymphs. Mortality of eggs and first instar nymphs was assessed by subtracting the number of surviving second instar nymphs from the initial egg counts.

Statistical Analyses

Dose-response data were analyzed by standard probit analysis, estimating LC50 values and the respective fiducial limits, slope and standard error (SE) of the regression line and the chi square value (x2) (SAS Institute 1994). The resistance ratios at 50% mortality (RR50) were calculated by dividing the LC50 value of each field population by that of the susceptible colony. Each experiment consisted of 4 replicates with sample size (N) of 309–642 B. tabaci eggs, not including those used for untreated controls. To assess and validate the consistency of the systemic bioassay, the entire experiment was repeated 3 times on different dates over a period of a month with the susceptible colony. Once the bioassay method was validated as described above, a single experiment with 4 replicates was conducted per field population. Comparisons of the fiducial limits of the LC50 values were used to determine significant differences between the laboratory colony and the field colonies as well among the field colonies. The slopes of the laboratory colony and the field populations were also compared to test for differences among populations within years using analyses of covariance (Proc ANCOVA) (SAS Institute 1994).

RESULTS

The systemic bioassay for chlorantraniliprole timed at the egg stage and using the susceptible colony provided repeatable results in 3 experiments in 2008 with LC50 values ranging from 0.0173 to 0.0522 mg ai L-1, and slopes from 1.154 to 1.373. The data, therefore, were pooled yielding a pooled LC50 and slope of 0.033 mg ai L-1 and 1.186, respectively (Table 1). In 2009, the susceptible colony, using the stabilization period, generated a LC50 and slope of 0.182 and 0.972, correspondingly.

Probit analyses of the mortality data of field populations collected from 5 commercial tomato farms in Southern Florida during the spring of 2008 and 3 during the spring of 2009 (GCC-EV-Tom, GCC #4, and GCC-BW) indicated no difference in susceptibility compared with the laboratory colony (Table 1). LC50 and slope values ranged from 0.016 to 0.046 mg ai L-1, and 0.889 to 1.595, respectively. The fiducial limits of the LC50 values of the laboratory colony and those of the field colonies overlapped, indicating no significant difference. The RR50 values of field colonies ranged from 0.496 to 1.377, also indicating no differences (Table 1). The slopes also did not differ significantly (F8,62 = 0.01; P = 1.00).

TABLE 1.

BASELINE SUSCEPTIBILITY OF BEMISIA TABACI FIELD-COLLECTED POPULATIONS FROM SOUTHERN FLORIDA TO CHLORANTRANILIPROLE USING A CUT COTTON STEM, SYSTEMIC UPTAKE BIOASSAY TIMED AT THE EGG STAGE IN THE LABORATORY IN 2008 AND 2009.

t01_1002.gif

The last 3 field populations collected during the spring of 2009 (Devil's Garden, Homestead #1, and GCC #2) were evaluated following a stabilization period (cut stems allowed to stay in water for 24 h prior to introducing the insecticide) and compared to the laboratory colony that was similarly evaluated. The LC50 value for the laboratory colony for a single bioassay was higher than when a stabilization period was not used. The LC50 values for these field populations are also higher than those not receiving the stabilization period, ranging from 0.117 to 0.251 mg ai L-1 although the slope ranged from 0.885 to 1.395, which was comparable to the slope of the populations treated with no stabilization period (Table 1). We speculate that the stabilization period causes plants to be uniformly saturated with water, thus reducing insecticide uptake in the plants and increasing the LC50 values as a response. Nevertheless, the probit analyses indicated no difference in susceptibility of the field populations compared to the laboratory colony. The fiducial limits of the LC50 values of the laboratory and field colonies overlapped supporting this conclusion. The RR50 values of the field populations were also low, ranging from 0.645 to 1.381 (Table 1). In addition, the slopes did not differ significantly among the laboratory and field populations (F3,27 = 0.04; P = 0.99).

DISCUSSION

The systemic bioassay for estimating susceptibility of B. tabaci to chlorantraniliprole proved to be consistent in several experiments with the susceptible laboratory colony. The susceptible colony has been in laboratory culture for almost 20 yr with no insecticide contact and without field introduction of whiteflies. Thus, the baseline results for this laboratory colony will be a key element for monitoring changes in susceptibility to chlorantraniliprole in field populations in time and space. Likewise, the analyses of the results of field populations demonstrated similar susceptibility to the laboratory population, which indicates that chlorantraniliprole has no cross-resistance to insecticides currently being used for whitefly control in Florida. Although chlorantraniliprole was registered in Aug 2008 and the field populations were collected from Apr to Jun in 2008 and in the spring of 2009, they showed high level of susceptibility to this insecticide. The lower mortality values in the last 3 populations analyzed in 2009 is attributed to the implementation of the stabilization period, causing less insecticide uptake by the cut seedlings. This step is considered key and a methodology upgrade that was incorporated later in this study to standardize amount of insecticide absorbed by each of the plants in the experiment. Similar results were found, using the same bioassay method, in a parallel study carried out at the University of Arizona, which was part of the team to develop baseline susceptibility data to chlorantraniliprole and cyantraniliprole (Li et al. 2012). The LC50 value in the present study, using the stabilization period, for the susceptible laboratory colony was of 0.182 mg ai L-1 compared to 0.179 mg ai L-1 reported by University of Arizona (Li et al. 2012) (Table 1).

Chlorantraniliprole has demonstrated excellent control of a broad-spectrum of Lepidopteran crop pests, including the families Crambidae (Ghidiu et al. 2009), Gelechiidae (Astor & Seals 2009), Noctuidae (Hardke et al. 2011), Pieridae (Dhawan 2010), Plutellidae (Wang et al. 2010), Psychidae (Rhaind & Sadof 2009), Pyralidae (Yang et al. 2010), and Tortricidae (Loriatti et al. 2009). It has also shown evidence of excellent control on insects of other orders such as Diptera [Tephritidae (Teixeira et al. 2008), Tipulidae (Peck et al. 2008), and Agromyzidae (Conroy et al. 2008)]; Coleoptera [Chrysomelidae (Tang et al. 2009), Curculionidae (Reding & Ranger 2011), and Scarabaeidae (Koppenhöfer & Fuzy 2008)]; Homopterans [Delphacidae (Wang et al. 2009) and Pseudococcidae (Dhawan et al. 2008)]; and Isoptera [Rhinotermitidae (Spomer & Kamble 2011)]. In addition, chlorantraniliprole has exhibited activity against whitefly populations (Homoptera: Aleyrodidae) in laboratory and in the field as well as suppression of transmission of the begomovirus TYLCV (Portillo et al. 2008; Schuster et al. 2008). Chlorantraniliprole also has shown safety to non-target arthropods, including pollinators, parasitoids and predatory insects and mites, and synergistic effects with an entomopathogenic nematode for controlling white grubs (Dinter et al. 2008; DuPont 2008; Koppenhöfer & Fuzy 2008; Preetha et al. 2009; Brugger et al. 2010; Shaw & Wallis 2010; Gradish et al. 2010, 2011). Thus, chlorantraniliprole is a promising tool as part of an integrated pest management program for B. tabaci, particularly where whiteflies have already developed resistance to other insecticide groups (Cahill et al. 1996a, b, c; Palumbo et al. 2001; Toscano et al. 2001; Li et al. 2003; Horowitz et al. 2007). The baseline information developed in the present study will be an essential component of a resistance management program and will help ensure the continued viability of chlorantraniliprole for B. tabaci management.

ACKNOWLEDGMENTS

The authors wish to express their appreciation to Leon Lucas (Glades Crop Care), Henry Yonce (KAC Agricultural Research) and Sarah Hornsby (Agricultural Crop Consulting) for identifying and/or collecting sweetpotato whitefly samples for monitoring. Appreciation is also expressed to DuPont Crop Protection for providing funding for the study.

REFERENCES CITED

1.

E. Astor , and D. De Scals 2009. The control of Tuta absoluta with insecticides compatible with integrated pest management programmes and the prevention of resistance. Agricola Vergel 28: 492–495. Google Scholar

2.

J. K. Brown , D. R. Frohlich , and R. C. Rosell 1995. The sweetpotato or silverleaf whiteflies: biotypes of Bemisia tabaci or a species complex? Annu. Rev. Entomol. 40: 511–534. Google Scholar

3.

K. E. Brugger , P. G. Cole , I. C. Newman , B. Scholz , P. Suvagia , G. Walker , and T. G. Hammond 2010. Selectivity of chlorantraniliprole to parasitoid wasps. Pest Mgt. Sci. 66: 1075–1081. Google Scholar

4.

R. Caballero , S. Cyman , D. J. Schuster , H. E. Portillo , and R. Slater 2013. Baseline susceptibility of Bemisia tabaci (Genn.) Biotype B in southern Florida to Cyantraniliprole. Crop Prot. 44: 104–108. Google Scholar

5.

M. Cahill , F. J. Byrne , K. Gorgan , I. Denholm , and A. L. Devonshire 1996a. Pyrethroid and organophosphate resistance in Bemisia tabaci (Homoptera: Aleyrodidae). Bull. Entomol. Res. 85: 181–187. Google Scholar

6.

M. Cahill , K. Gorman , S. Day , L. Denholm , A. Elbert , and R. Nauen 1996b. Baseline determination and detection of resistance to imidacloprid in Bemisia tabaci (Homoptera: Aleyrodidae). Bull. Entomol. Res. 86: 343–349. Google Scholar

7.

M. Cahill , W. Jarvis , K. Gorman , and I. Denholm 1996c. Resolution of baseline responses and documentation of resistance to buprofezin in Bemisia tabaci (Homoptera: Aleyrodidae). Bull. Entomol. Res. 86: 117– 122. Google Scholar

8.

L. Conroy , C. D. Scott-Dupree , C. R. Harris , G. Murphy , and A. B. Broadbent 2008. Susceptibility of two strains of American Serpentine Leafminer (Liriomyza trifolii (Burgess)) to registered and reduced risk insecticides in Ontario. J. Entomol. Soc. Ont. 139: 41– 47. Google Scholar

9.

D. Cordova , E. A. Benner , M. D. Sacher , J. J. Rauh , J. S. Sopa , G. P. Lahm , T. P. Selby , T. M. Stevenson , T. Caspar , J. J. Ragghianti , S. Gutteridge , D. F. Rhoades , L. H. Wu , R. M. Smith , and Y. Tao 2007. Anthranilic diamides: A new class of highly potent ryanodine receptor activators. Biophys. J. 87A. Google Scholar

10.

D. Cordova , E. A. Benner , M. D. Sacher , J. J. Rauh , J. S. Sopa , G. P. Lahm , T. P. Selby , T. M. Stevenson , L. Flexner , S. Gutteridge , D. F. Rhoades , L. Wu , R. M. Smith , and Y. Tao 2006. Anthranilic diamides: A new class of insecticides with a novel mode of action, ryanodine receptor activation. Pestic. Biochem. Phys. 84: 196–214. Google Scholar

11.

A. K. Dhawan , K. Amandeep , S. Rajinder , M Shaonpius , and K. Gurpreet 2010. Relative toxicity of novel insecticides against cabbage butterfly, Pieris brassicae Linnaeus. J. Insect Sci. 23: 318–321. Google Scholar

12.

A. K. Dhawan , S. Sarika , S. Kamaldeep , and M. Bharathi 2008. Toxicity of some new insecticides against Phenacoccus solenopsis (Tinsley) [Hemiptera: Pseudococcidae] on cotton. J. Insect Sci. 21: 103–105. Google Scholar

13.

A. Dinter , K. Brugger , A. Bassi , N-M. Frost , and M. D. Woodward 2008. Chlorantraniliprole (DPX-E2Y45, DuPont™ Rynaxypyr®, Coragen® and Altacor® insecticide) - a novel insecticide - demonstrating low toxicity and low risk for beneficial insects and predatory mites. IPM IOBC Bull. 35: 128–136. Google Scholar

14.

Dupont. 2008. DuPont™ Coragen® insect control powered by Rynaxypyr. Dupont Technical Bulletin.  http://www2.dupont.com/Production_Agriculture/en_US/assets/downloads/pdfs/K-14833_Coragen_Tech_Bulletin.pdf. Accessed 24 Jun 2013. Google Scholar

15.

G. M. Ghidiu , D. L. Ward , and G. S. Rogers 2009. Control of European corn borer in bell peppers with chlorantraniliprole applied through a drip irrigation system. Intl. J. Vegetable Sci. 15: 193–201. Google Scholar

16.

A. E. Gradish , C. D. Scott-dupree , L. Shipp , C. R. Harris , and G. Ferguson 2010. The effect of reduced risk pesticides for use in greenhouse vegetable production on bumble bees (Bombus impatiens Cresson). Pest Mgt. Sci. 66: 142–146. Google Scholar

17.

A. E. Gradish , C. D. Scott-dupree , L. Shipp , C. R. Harris , and G. Ferguson 2011. Effect of reduced risk pesticides on greenhouse vegetable arthropod biological control agents. Pest Mgt. Sci.67: 82–86. Google Scholar

18.

J. T. Hardke , J. H. Temple , B. R. Leonard , and R. E. Jackson 2011. Laboratory toxicity and field efficacy of selected insecticides against Fall Armyworm (Lepidoptera: Noctuidae). Florida Entomol. 94: 272–278. Google Scholar

19.

A. R. Horowitz , I. Denholm , and S. Morin 2007. Resistance to insecticides in the TYLCV vector, Bemisia tabaci , pp. 305–325 In H. Czosnek [ed.], Tomato Yellow Leaf Curl Virus Disease, Management, Molecular Biology and Breeding for Resistance. Springer, Dordrecht, The Netherlands. Google Scholar

20.

IRAC. 2012. IRAC MoA Classification Scheme, Version 7.2. IRAC International MoA Working Group. 23 pp.  http://www.irac-online.org/content/uploads/MoA-classification.pdf. Accessed 14 Jun 2013. Google Scholar

21.

A. M. Koppenhöfer , and E. M. Fuzy 2008. Effect of the anthranilic diamide insecticide, chlorantraniliprole, on Heterorhabditis bacteriophora (Rhabditida: Heterorhabditida) efficacy against white grubs (Coleoptera: Scarabaeidae). Biol. Control 45: 93–102. Google Scholar

22.

J. B. Kring , D. J. Schuster , J. F. Price , and G. W. Simone 1991. Sweetpotato whitefly-vectored geminivirus on tomato in Florida. Plant Dis. 75: 1186. Google Scholar

23.

G. P. Lahm , T. P. Selby , J. H. Freudenberger , T. M. Stevenson , B. J. Myers , G. Seburyamo , B. K. Smith , L. Flexner , C. E. Clark , and D. Cordova 2005. Insecticidal anthranilic diamides: A new class of potent ryanodine receptor activators. Bioorg. Med. Chem. Lett. 15: 4898–4906. Google Scholar

24.

G. P. Lahm , T. M. Stevenson , T. P. Selby , J. H. Freudenberger , D. Cordova , L. Flexner , C. A. Bellin , C. M. Dubas , B. K. Smith , K. A. Hughes , J. G. Hollingshaus , C. E. Clark , and E. A. Benner 2007. Rynaxypyr®: A new insecticidal anthanilic diamide that acts as a potent and selective ryanodine receptor activator. Bioorg. Med. Chem. Lett. 17: 6274– 6279. Google Scholar

25.

G. P. Lahm , D. Cordova , and J. D. Barry 2009. New and selective ryanodine receptor activators for insect control. Bioorg. Med. Chem. 17: 4127–4133. Google Scholar

26.

J. Legocki , L Polec , and K. Zelechowski 2008. Contemporary trends in development of active substances possessing the pesticidal properties: ryanodine-receptor targeting insecticides. Pesticides 3–4: 15–26. Google Scholar

27.

X. Li , B. A. Degain , V. S. Harpold , P. G. Marçon , R. L. Nichols , A. J. Fournier , S. E. Naranjo , J. C. Palumbo , and P. C. Ellsworth 2012. Baseline susceptibilities of B- and Q-biotype Bemisia tabaci to anthranilic diamides in Arizona. Pest Mgt. Sci. 68: 83– 91. Google Scholar

28.

A. Y. Li , T. J. Dennehy , and R. L. Nichols 2003. Baseline susceptibility and development of resistance to pyriproxyfen in Bemisia argentifolii (Homoptera: Aleyrodidae) in Arizona. J. Econ. Entomol. 96: 1307–1314. Google Scholar

29.

C. Loriatti , G. Anfora , G. Angeli , V. Mazonni , and F. Trona 2009. Effects of chlorantraniliprole on eggs and larvae of Lobesia botrana (Denis & Schiffermüller) (Lepidoptera: Tortricidae). J. Econ. Entomol. 65: 717–722. Google Scholar

30.

J. C. Palumbo , A. R. Horowitz , and N. Prabhaker 2001. Insecticidal control and resistance management for Bemisia tabaci. Crop Prot. 20: 739–765. Google Scholar

31.

D. C. Peck , D. Olmstead , and A. Morales 2008. Application timing and efficacy of alternatives for the insecticidal control of Tipula paludosa Meigen (Diptera: Tipulidae), a new invasive pest of turf in the northeastern United States. Pest Mgt. Sci. 64: 989–1000. Google Scholar

32.

J. E. Polston , R. J. McGovern , and L. G. Brown 1999. Introduction of tomato yellow leaf curl virus in Florida and implications for the spread of this and other geminiviruses of tomato. Plant Dis. 83: 984–988. Google Scholar

33.

H. Portillo , P. C. Marçon , R. W. Williams , D. Tamayo , and D. W. Sherrod 2008. Coragen™ SC (DPXE2Y45): a novel anthranilamide insecticide: pest spectrum with emphasis on whitefly control in vegetables. J. Insect Sci. 8: 39. Google Scholar

34.

G. Preetha , J. Stanley , S. Suresh , S. Kuttalam , and R. Samiyappan 2009. Toxicity of selected insecticides to Trichogramma chilonis: assessing their safety in the rice ecosystem. Phytoparasitica 37: 209–215. Google Scholar

35.

J. F. Price 1987. Controlling a new pest. Greenhouse Grower 5: 72–73. Google Scholar

36.

M. E. Reding , and C. M. Ranger 2011. Systemic insecticides reduce feeding, survival, and fecundity of adult black vine weevils (Coleoptera: Curculionidae) on a variety of ornamental nursery crops. J. Econ. Entomol. 104: 405–413. Google Scholar

37.

M. Rhainds , and C. Sadof 2009. Control of Bagworms (Lepidoptera: Psychidae) using contact and soilapplied systemic insecticides. J. Econ. Entomol. 102: 1164–1169. Google Scholar

38.

SAS Institute . 1994. SAS/STAT User's Guide, version 6 (4th edition). SAS Institute, Cary, NC, USA. Google Scholar

39.

D. J. Schuster 2007. Whitefly resistance update, pp. 23– 27 In G. P. Whidden and E. Simmone [eds.], Florida Tomato Inst. Proc. Univ. Florida, Gainesville, PRO 524. Google Scholar

40.

D. J. Schuster , P. H. Everett , J. F. Price , and J. B. Kring 1989. Supression of the sweetpotato whitefly on commercial fresh market tomatoes. Proc. Fla. State Hort. Soc. 102: 374–379. Google Scholar

41.

D. J. Schuster , R. Mann , and P. R. Gilreath 2006. Whitefly resistance update and proposed mandated burn down rule, pp. 24–28 In G. P. Whidden and K. Cushman [eds.], Florida Tomato Inst. Proc. Univ. Florida, Gainesville, PRO 523. Google Scholar

42.

D. J. Schuster , R. S. Mann , M. Toapanta , R. Cordero , S. Thompson , S. Cyman , A Shurtleff , and R. F. Morris II 2010. Monitoring neonicotinoid resistance in biotype B of Bemisia tabaci in Florida. Pest Mgt. Sci. 66: 186–195. Google Scholar

43.

D. J. Schuster , T. F. Mueller , J. B. Kring , and J. F. Price 1990. Relationship of the sweetpotato whitefly to a new tomato disorder in Florida. HortScience 25: 1618–1620. Google Scholar

44.

D. J. Schuster , N. A. Peres , R. W. Williams , P. C. Marçon , and H. E. Portillo 2008. DuPont Rynaxypyr™ (DPX-E2Y45): a novel anthranilamide insecticide for managing Bemisia tabaci and interfering with transmission of Tomato Yellow Leaf Curl Virus on tomato transplants. J. Insect Sci. 8: 43. Google Scholar

45.

D. J. Schuster , and S. Thompson 2001. Monitoring susceptibility of the silverleaf whitefly to imidacloprid, pp. 16–18 In G. P. Whidden and C. S. Vavrina [eds.], Florida Tomato Inst. Proc. Univ. Florida, Gainesville, PRO-518. Google Scholar

46.

D. J. Schuster , and S. Thompson 2004. Silverleaf whitefly resistance management update, pp. 19–25 In G. P. Whidden and W. H. Stall [eds.], Florida Tomato Inst. Proc. Univ. Florida, Gainesville, PRO 521. Google Scholar

47.

D. J. Schuster , S. Thompson , and P. R. Gilreath 2003. What's up with all these whiteflies? pp. 12–19 In G. P. Whidden and W. H. Stall [eds.], Florida Tomato Inst. Proc. Univ. Florida, Gainesville, PRO-520. Google Scholar

48.

D. J. Schuster , S. Thompson , P. A. Stansly , and J. Conner 2002. Update on insecticides for whitefly and leafminer control, pp. 51–60 In G. P. Whidden and C. S. Vavrina [eds.], Florida Tomato Inst. Proc. Univ. Florida, Gainesville, PRO-519. Google Scholar

49.

P. W. Shaw , and D. R. Wallis 2010. Susceptibility of the European earwig, Forficula auricularia, to insecticide residues on apple leaves. N. Z. Plant Protect-SE 63: 55–59. Google Scholar

50.

N. A. Spomer , and S. T. Kamble 2011. Temporal changes in chlorantraniliprole and indoxacarb in four midwestern soils and bioefficacy against the eastern subterranean termite (Isoptera: Rhinotermitidae). J. Econ. Entomol. 104: 990–1001. Google Scholar

51.

T. Tang , D. Liu , G Ma, X Liu , and C. Wei 2009. Control effect of 30% chlorantraniliprole, thiamethoxam SC drenched in seedbed on insect pests of cabbage (Brassica oleracea L. var. capitata L.) plants. China Vegetables 22: 63–66. Google Scholar

52.

L. A. F. Teixeira , L. J. Gut , J. C. Wise , and R. Isaacs 2008. Lethal and sublethal effects of chlorantraniliprole on three species of Rhagoletis fruit flies (Diptera: Tephritidae). Pest Mgt. Sci. 65: 137–143. Google Scholar

53.

N. C. Toscano , N. Prabhaker , S. J. Castle , and T. J. Henneberry 2001. Inter-regional differences in baseline toxicity of Bemisia argentifolii (Homoptera: Aleyrodidae) to the two insect growth regulators, buprofezin and pyriproxyfen. J. Econ. Entomol. 94: 1538– 1546. Google Scholar

54.

USDA-NASS. 2012. Florida Agriculture Statistical Bulletin. Vegetables  http://www.nass.usda.gov/Statistics_by_State/Florida/Publications/Vegetables/apv/vegapv12.pdf Accessed 24. Jun 2013. Google Scholar

55.

Y. M. Wang , Y. L. Zhang , X. Y. Wu , X. L. Lu , S. Lu , and C. M. Yan 2009. Effects of several pesticides on controlling Laodelphax striatellus and Cnaphalocrocis medinalis and killing spiders. Acta Agric. Shanghai 25: 147–150. Google Scholar

56.

X. L. Wang , X. Y. Li , A. D. Shen , and Y. D. Wu 2010. Baseline susceptibility of the Diamondback moth (Lepidoptera: Plutellidae) to chlorantraniliprole in China. J. Econ. Entomol. 103: 843–848. Google Scholar

57.

M. F. Wilks , R. A. Brown , K. S. Bentley , and D. Cordova 2008. On the horizon - New pesticides, new applications, predicting future risks from today's experiments. Clin. Toxicol. 46: 405–405. Google Scholar

58.

L. W. Yang , J. Z. Chen , Y. T. Dai , L. W. Ding , and J. W. Yang 2010. Control effect of three new amide pesticides on rice leaf rolder, Cnaphalocrocis medinalis, at the booting stage of rice. Chinese Bull. Entomol. 47: 393–395. Google Scholar
Rafael Caballero, Sabrina Cyman, and David J. Schuster "Baseline Susceptibility of Bemisia tabaci, Biotype B (Hemiptera: Aleyrodidae) to Chlorantraniliprole in Southern Florida," Florida Entomologist 96(3), 1002-1008, (1 September 2013). https://doi.org/10.1653/024.096.0338
Published: 1 September 2013
JOURNAL ARTICLE
7 PAGES


SHARE
ARTICLE IMPACT
Back to Top