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Field-Evolved Resistance in Corn Earworm to Cry Proteins Expressed by Transgenic Sweet Corn

  • Galen P. Dively,

    Affiliation Department of Entomology, University of Maryland, College Park, Maryland, United States of America

  • P. Dilip Venugopal ,

    Affiliations Department of Entomology, University of Maryland, College Park, Maryland, United States of America, American Association for the Advancement of Science - Science and Technology Policy Fellowship Program, Transportation and Climate Division, Office of Transportation & Air Quality, United States Environmental Protection Agency, District of Columbia, United States of America

  • Chad Finkenbinder

    Affiliation Benzon Research Inc., Carlisle, Pennsylvania, United States of America


17 Aug 2017: Dively GP, Venugopal PD, Finkenbinder C (2017) Correction: Field-Evolved Resistance in Corn Earworm to Cry Proteins Expressed by Transgenic Sweet Corn. PLOS ONE 12(8): e0183637. View correction



Transgenic corn engineered with genes expressing insecticidal toxins from the bacterium Bacillus thuringiensis (Berliner) (Bt) are now a major tool in insect pest management. With its widespread use, insect resistance is a major threat to the sustainability of the Bt transgenic technology. For all Bt corn expressing Cry toxins, the high dose requirement for resistance management is not achieved for corn earworm, Helicoverpa zea (Boddie), which is more tolerant to the Bt toxins.

Methodology/Major Findings

We present field monitoring data using Cry1Ab (1996–2016) and Cry1A.105+Cry2Ab2 (2010–2016) expressing sweet corn hybrids as in-field screens to measure changes in field efficacy and Cry toxin susceptibility to H. zea. Larvae successfully damaged an increasing proportion of ears, consumed more kernel area, and reached later developmental stages (4th - 6th instars) in both types of Bt hybrids (Cry1Ab—event Bt11, and Cry1A.105+Cry2Ab2—event MON89034) since their commercial introduction. Yearly patterns of H. zea population abundance were unrelated to reductions in control efficacy. There was no evidence of field efficacy or tissue toxicity differences among different Cry1Ab hybrids that could contribute to the decline in control efficacy. Supportive data from laboratory bioassays demonstrate significant differences in weight gain and fitness characteristics between the Maryland H. zea strain and a susceptible strain. In bioassays with Cry1Ab expressing green leaf tissue, Maryland H. zea strain gained more weight than the susceptible strain at all concentrations tested. Fitness of the Maryland H. zea strain was significantly lower than that of the susceptible strain as indicated by lower hatch rate, longer time to adult eclosion, lower pupal weight, and reduced survival to adulthood.


After ruling out possible contributing factors, the rapid change in field efficacy in recent years and decreased susceptibility of H. zea to Bt sweet corn provide strong evidence of field-evolved resistance in H. zea populations to multiple Cry toxins. The high adoption rate of Bt field corn and cotton, along with the moderate dose expression of Cry1Ab and related Cry toxins in these crops, and decreasing refuge compliance probably contributed to the evolution of resistance. Our results have important implications for resistance monitoring, refuge requirements and other regulatory policies, cross-resistance issues, and the sustainability of the pyramided Bt technology.


Transgenic crops engineered with genes expressing insecticidal toxins from the bacterium Bacillus thuringiensis (Berliner) (Bt) are now a major tool in insect pest management, with increasing global adoption since commercial availability in 1996 [1]. Bt transgenic technology is safe for human health, and may provide multi-fold benefits including reductions in pests and pesticide usage, and increases in yield, profits and food security [29]. In the U.S., single-gene and pyramided Bt crops constituted 81% of the total 35.6 million ha of maize (corn), Zea mays L., planted in 2015, and 84% of the total 3.6 million ha of planted cotton Gossypium sp. L. [10,11]. Bt toxins targeting lepidopteran pests in these crops include Cry1Ab, Cry1Ac, Cry1A.105, Cry1F, Cry2Ab2, Cry2Ae and Vip3A.

With the widespread use of Bt crops, insect resistance is the major threat to the sustainability of the Bt transgenic technology. Thus, an insect resistance management (IRM) plan aimed at delaying the onset of resistance is required by the U. S. Environmental Protection Agency (EPA) for commercial registration of Bt crops in the U.S [12]. As the key component of IRM, high dose-refuge strategies have been widely adopted targeting specific insect pests, which deploy a high toxin expression to kill nearly all heterozygous resistant individuals. When used in combination with non-Bt crops grown in proximity or amidst Bt crops as refuges, this strategy allows survival and mating of susceptible insects with Bt resistant insects, thereby keeping the resistant allele frequency low [13]. For single-gene Bt corn hybrids, primarily targeting European corn borer, Ostrinia nubilalis (Hübner), EPA mandates a 20% and 50% structured refuge in the corn belt and cotton growing regions, respectively. Also, the refuge-in-the-bag (RIB) strategy with a 5% refuge requirement (95% Bt) is now approved for hybrids expressing multiple pyramided Bt proteins for lepidopteran control in the corn belt [14]. The RIB strategy primarily aims to manage evolution of resistance in O. nubilalis (Hübner), but not corn earworm, Helicoverpa zea (Boddie). For this reason, there still is a 20% structured refuge requirement for Bt corn with no option for the RIB strategy in the southern U.S. which faces high H. zea population pressure [15] and additional selection from Bt cotton.

While IRM for Bt corn has proved effective in delaying O. nubilalis resistance, reports of other insect pests developing resistance to the insecticidal toxins are on the rise (see [16,17] for recent reviews). Since 2002, field-evolved resistance to Bt crops [sensu [16,18]; > 50% resistant individuals and reduced efficacy] is reported for five major insect pests across different countries [17]. This includes the fall armyworm, Spodoptera frugiperda (J.E. Smith) for Cry1F in Puerto Rico, Brazil and continental U.S. [1923] and Cry1Ab in Brazil [24]; maize stalk borer, Busseola fusca (Fuller) for Cry1Ab in South Africa [25]; pink bollworm, Pectinophora gossypiella (Saunders) for Cry1Ac in India [26]; Western corn rootworm, Diabrotica v. virgifera LeConte for Cry3Bb and mCry3A in U.S. [2729]; and corn earworm, H. zea (Boddie) for Cry1Ac in U.S [16, 30]. Reports of field-evolved resistance by H. zea to Cry1Ac was refuted by Moar et al. [31], to which Tabashnik et al. [32] responded with further confirmations on the initial report. H. zea may also be developing resistance to Cry1Ab in field corn [33]. Additionally, cross-resistance can occur among closely related Cry toxins, particularly those selected for pest resistance in single-gene Bt crops, which can likely lead to more rapid pest resistance development in crops expressing multiple pyramided toxins [22,3437]. Previous reports have shown cross-resistance between the Cry1A proteins (1Ab, 1Ac, Cry1A.105) in H. zea [38,39]. Santos-Amaya et al. [40] found that Cry1F resistant S. frugiperda selected in Bt corn was also highly resistant to Bt cotton expressing Cry1Ac and Cry1f toxins, and Yang et al. [41] reported that a laboratory selected strain of S. frugiperda to Cry1A.105 and Cry2Ab2 showed cross-resistance to Cry1F. Recently, Hernandez-Rodriguez et al [42] demonstrated that O. nubilalis and S. frugiperda shared midgut binding sites for Cry1A.105, Cry1Ab and Cry1Ac, implying cross resistance between these proteins.

Registrants of Bt corn are also required by the EPA to annually monitor potential changes in susceptibility of target insect species to Bt toxins in order to detect the evolution of resistance before field efficacy fails [43]. To monitor susceptibility changes, the performance and mortality of the progeny of field-collected insects to a Bt toxin is tested at diagnostic concentrations, and compared to a known range of baseline susceptibility [4446]. A significant decrease in susceptibility of a population based on this approach is viewed as genetically mediated and confirmation of field-evolved resistance, as defined by Tabashnik et al. [43]. However, when field populations evolve resistance to Bt toxins, decreased susceptibility to Bt crops, resulting in a reduction in field efficacy is usually expected [43]. Moar et al. [31] defined field-evolved resistance based on a change in field efficacy, documented as an increased ability of a target pest to feed and complete development. Such a definition of field-evolved resistance incorporates the outcomes of genetically mediated changes in sensitivity of the target pest to Bt toxins, such as the potential for incomplete resistance and fitness costs where pest feeding on Bt crops increases but development to adult is delayed or incomplete [31]. In addition to the laboratory bioassays to determine resistance, comparison of target pest susceptibility and control efficacy in paired fields of Bt and non-Bt crops is a practical method to monitor evolution of resistance in the field [31,47]. Resistance definition by Tabashnik et al. [16,18], which we follow in this study, comprises different categories of resistance, including the field efficacy changes as a basis for resistance development.

H. zea is the key pest of sweet corn and polyphagous in many agricultural crop systems, and it is capable of migrating long distances [15]. For sweet corn production, Attribute (expressing Cry1Ab toxin, event Bt11) and Attribute II (expressing Cry1Ab and Vip3A, event MIR162) hybrids from Syngenta Seeds, and Performance Series (PS) hybrids (expressing the Cry1A.105 and Cry2Ab2 toxins, event MON89034) from Seminis Seeds are commercially available. For these Bt hybrids, which represents <1% of the corn hectares grown in the U.S., there is no refuge requirement. Growers are required to destroy the stalks following harvest. For all Bt corn expressing Cry toxins, the high dose requirement for IRM is achieved for O. nubilalis, but it is not true for H. zea which is more tolerant to the Bt toxins [48]. In 2003, Horner et al. [49] reported that Bt field corn (Cry1Ab, event MON810) suppressed the establishment and development of H. zea to late instars by at least 75%. They suggested that this moderate dose effect might increase the risk of evolution of resistance in areas where Cry1Ab expressing corn is widely adopted and H. zea overwinters successfully. Efficacy of single event Cry1Ab sweet corn for controlling H. zea was highly variable during 2008–2011, (for example, 8.0%– 73% clean ears in Maryland; [50,51]) with increasing concerns over lack of H. zea control by Cry1Ab in Bt sweet corn [51].

Here we present findings from 21 years of monitoring changes in Cry1Ab susceptibility to H. zea and field efficacy in Bt sweet corn as an in-field screen. We hypothesized that a change in control efficacy since its commercial availability in 1996 is evidence of field-evolved resistance of H. zea to Cry1Ab toxins. We also provide data on recent changes in field efficacy of Cry1A.105+Cry2Ab2 sweet corn, suggesting resistance development in H. zea to multiple Cry toxins. Further, we investigated patterns of H. zea population abundance, and differences among Bt hybrids for the efficacy parameters (as surrogate for toxin expression among Bt hybrids) as they might affect control efficacy. Finally, supportive information from laboratory bioassays provide preliminary evidence of susceptibility changes by comparing weight gain, toxicity responses, and fitness characteristics of a H. zea strain reared from surviving larvae on Bt sweet corn with a susceptible strain.


Ethics statement

No endangered or protected species were involved in the study. Study was conducted at the University of Maryland Research and Education farm facilities for which we had permission to access and collect data.

Study design

Venette et al. [47] proposed the use of sentinel Bt sweet corn as an in-field screen to monitor evolution of target pest resistance and overall efficacy of Bt corn. Sweet corn, Zea mays var. saccharata, represents an ideal host plant for monitoring early shifts in H. zea susceptibility and can effectively function as an in-field diagnostic dose for several reasons. First, when first introduced commercially, both Attribute and PS hybrids provided greater than 95% control efficacy against H. zea in most field trials [5053]. Second, late season plantings of sweet corn are highly attractive to H. zea moths during the silking and ear development period, and significantly more infested than populations found in field corn, thus reducing the sample size of ears required to statistically detect changes in H. zea damage. For late plantings devoid of insecticidal treatments, infestation of most ears of non-Bt hybrids by H. zea is likely [47]. Unlike field corn, sweet corn is harvested at a premature stage, thus toxin expression is consistently high throughout the crop cycle and generally higher in the silk and kernel tissues than in Bt field corn. Lastly, it is relatively easy to quantify changes in the incidence and severity of ear damage in sweet corn as a measure of control efficacy.

Sentinel plots of Bt sweet corn hybrids paired with non-Bt isogenic hybrids were established each year during 1996 to 2016 to evaluate H. zea infestations in ears as a direct measure of control efficacy and indication of changes in Bt toxin susceptibility. Cry1Ab hybrids were commercially available in 1996 and evaluated during all years, whereas Cry1A.105+Cry2Ab2 hybrids were developed later and included in studies from 2010 to 2016. Additionally, we evaluated the field performance of pyramided Cry1Ab+Vip3A hybrids in plots planted each year since 2008, alongside other Bt sweet corn types at the same locations. During each year, one or two late plantings were established at five University of Maryland Research and Education farm facilities—Salisbury and Queenstown on the Eastern Shore of Maryland, and at Upper Marlboro (38.86° N, 76.78° W), Beltsville (39.01° N, 76.83° W) and Clarksville (39.25° N, 76.93° W) in central Maryland. Plots were seeded during June at each farm location to encourage high infestations of H. zea that typically occur in late August during silking and ear development [54,55]. One replicate pair of Bt and non-Bt plots were established at most locations; however, replicated plots of each hybrid were included during some years and locations. Plots ranged in size from 6 to 12 rows 15–30 m long and were maintained according to commercial production recommendations, except no insecticides were applied.

Control efficacy assessments

All plots were sampled to assess ear damage during mid-August through mid-September when ears reached fresh market maturity (usually 18–21 days after the onset of silking). We examined 50–100 primary ears from the center rows of each plot, depending on plot size and level of infestation. Ears were removed and either brought back to the laboratory for processing or data were recorded directly from husked ears in situ. The following variables were recorded as measures of control efficacy: percentage of ears damaged by H. zea, mean kernel area consumed, and mean instar stage (henceforth damage, consumption, and instar, respectively). Each ear was carefully examined for kernel injury and recorded by pest species. The total kernel area consumed (cm2) was visually estimated as a measure of the extent of ear damage. Technicians were trained to estimate injured kernel area to ensure consistent and accurate data. A convenient reference used for estimation was the 0.5 cm2 cross-section of a standard pencil eraser. Damage greater than 0.5 cm2 was recorded to the nearest 0.5 cm2, but for very minor injury on a few kernels (<0.5 cm2; common on Bt ears), damage was recorded as 0.2 cm2. For calculating mean kernel consumption, we used only the data from damaged ears. The number of live and dead H. zea larvae found in each ear was recorded by instar. For ears with kernel damage but no larvae present, we assumed a late instar H. zea completed development if kernel area consumption was greater than 8 cm2 with heavy deposits of frass, discarded head capsules, and presence of an exit hole. In addition to the mean instar stage, we calculated the proportion of late instar (4th– 6th instars) found in Bt ears as another measure of larvae development. Fall armyworm, S. frugiperda (J.E. Smith), is not a major ear-invading pest in Maryland. However, when there was evidence of multi-species infestations without larvae present, we carefully examined for shed head capsules, differences in frass deposits, and characteristic feeding patterns to distinguish between S. frugiperda and H. zea damage. O. nubilalis damage was easily distinguished from that of H. zea by the characteristic frass and the tunneling injury going into the cob at the tip, side, or base of the ear.

For plantings with replicate plots of Bt and non-Bt hybrids, we used averages over the replicates to avoid pseudo-replication and conducted statistical analyses for each control efficacy variables (damage, instar, consumption and proportion of late instars). We analysed the comparative trends in each variable between Bt and non-Bt hybrids of each Bt type over the study period, except for the Cry1Ab+Vip3A sweet corn data which contained almost all zeros for each variable. Each analysis performed individual linear mixed models (LMM) based on restricted maximum likelihood (REML) assuming a normal error distribution except for proportion of large instar for Cry1A.105+Cry2Ab2 which was analysed through Gaussian GLMM (identity function). Statistical significance of the fixed effects in the LMMs was tested through Wald F tests with Kenward-Roger approximation, and for GLMM through Wald Χ2 test [56].

In each of these LMMs, damage, instar, consumption, and proportion of later instars were the response variables, interaction effect of year and treatment (Bt vs non-Bt) was the fixed effect, and the study site was included as a random effect to account for repeated measurement [56]. Where applicable, we square root transformed the data to conform to linear model assumptions. We tested for the interaction effect of year and treatment because it denotes significant slope differences between Bt and non-Bt hybrids.

Bioassays for resistance characterization in Helicoverpa zea field-collected populations

Insect collections.

Previously we had unsuccessfully attempted to establish a H. zea colony from larvae surviving Bt sweet corn during 2008–2012 to determine the extent of field-evolved resistance through laboratory bioassays. Procedural details and results of these attempts are available in S1 Appendix. In 2015 we collected surviving H. zea from two 0.2 h fields of Attribute sweet corn (hybrid ‘BC0805’, expressing Cry1Ab) at two University of Maryland Research and Education facilities. One field was planted on 25 June at Salisbury (38.37° N, 75.66° W), while the second was planted on 20 June at Queenstown (38.80° N, 76.17° W). Fields were planted late so that the attractive silking stages coincided with peak moth activity during late August. Each field was maintained according to commercial production recommendations, except no insecticides were applied. At about 18 days after first silking (late August), ears were husked open in situ at both locations to expose surviving H. zea larvae. We removed 1,200 5th and 6th instars from ears, transferred them to 1 oz plastic cups containing 1.5 ml of H. zea meridic diet, and brought back to the laboratory where they were reared individually at 25°C until pupation. Pupae were removed and surface sterilized in a 5% Clorox (8.25% sodium hypochlorite ai) solution for 3 min and rinsed in water. In September 2015, 600 pupae were shipped to Benzon Research Inc. (Carlisle, PA), where a breeding colony (henceforth UMD 2015 strain) was established and maintained using standard rearing methods [57] through two generations before bioassays were conducted. The Benzon laboratory also maintains a colony of susceptible H. zea strain that was used as a standard reference.

Tissue-incorporated bioassays.

Green leaf tissue was collected from Attribute sweet corn (hybrid ‘BC0805’) and its non-expressing isogenic hybrid ‘Providence’ at full tassel at the Beltsville study site. Two leaves above the ear were removed from a random sample of 20 plants of each type, cut into smaller sections, and dried as a composite sample in a freeze dryer. The lyophilized Bt and non-Bt tissue was then ground to a fine powder in a commercial grinder (IKA Works, Inc, Wilmington, DE) and kept at -80°C until used in bioassays. Eggs of the UMD 2015 and susceptible strains were obtained from Benzon Research and incubated in a growth chamber until hatch. Because eggs of the UMD 2015 strain exhibited delayed development, temperature regimes were manipulated to schedule larvae of the same size of each strain. The neonates were reared on a H. zea meridic diet (Southland Products, Lake Village, AR) until the early 2nd instar for testing.

Three bioassays, each with two replicates of eight concentrations of Bt leaf tissue, were conducted on different days (4 Feb, 23 Feb and 7 April), using larvae from the 3rd, 4th and 5th generations of the UMD 2015 strain, respectively. At each bioassay, 1200 ml of meridic diet (adjusted with more water to offset for the added leaf tissue) was prepared and cooled to 55°C. in a water bath. Pre-weighed quantities of the Bt and non-Bt powdered tissue were prepared in the following proportions: 1) 300 mg non-Bt, 2) 10 mg Bt plus 290 mg non-Bt, 3) 20 mg Bt plus 280 mg non-Bt, 4) 40 mg Bt plus 260 mg non-Bt, 5) 80 mg Bt plus 220 mg non-Bt, 6) 160 mg Bt plus 140 mg non-Bt, 7) 300 mg Bt, and 8) 600 mg Bt. With the exception of the last quantity, the amount of total leaf powder added to the diet was the same for each concentration to standardize the composition of the diet.

For each diet concentration, 25 ml of molten diet was drawn into a 60 cc syringe with a 4 ml dia opening at the tip. The cap was then placed over the tip and the plunger was pulled back and removed from the syringe. Starting with the non-Bt concentration, a pre-weighed quantity of the leaf powder was added to the diet through the open end of the syringe. The plunger was then re-inserted, and the mixture homogenized by shaking the syringe for 30 seconds, followed by firmly holding the syringe on a rubber platform of a vortex mixer for another 30 seconds. With the tip cap removed, the leaf powder-diet mixture of each concentration was dispensed to one 32-well section of a 128-well bioassay tray (C-D International). Approximately 1.5 ml of diet was added to each well. The dilutions by adding leaf tissue to 25 ml of diet resulted in relatively low exposure doses; for example, the diet incorporating 600 mg of powder contained approximately 2–3% Bt leaf tissue.

After the diet mixture cooled and solidified, one early 2nd instar (18–24 hours old) was placed in each well using a camel-hair brush. Each 16-well section of the bioassay tray was sealed with a perforated adhesive lid. The trays were held in a growth chamber at 25°C, L:D 14:10, and 40–60% RH. Each tray contained one replicate of the eight concentrations and was infested with larvae from either the UMD 2015 or susceptible H. zea strain. After seven days, live larvae within each row of four wells were pooled and weighed together. The average weight gain per larva was calculated by dividing the pooled weight by the number of larvae in the row group.

Leaf tissue-incorporated bioassays data was analysed through a quasi-Poisson GLM with average weight after a week of feeding as the response variable and, strain (UMD 2015 and susceptible), diet concentration, and the interaction as the fixed effects. If interaction term was significant, we performed post-hoc mean comparisons (α = 0.05; Bonferroni correction) of weight gain between UMD 2015 and susceptible strains for each level of the diet concentration.

Fitness costs of resistance evolution

Previous attempts to establish a H. zea colony from surviving larvae collected from Cry1Ab sweet corn failed, possible due to suspected fitness costs (see S2 Appendix). To address the fitness issue, the UMD 2015 and susceptible strains were reared under laboratory conditions and assessed simultaneously for egg hatch, survival from egg to adult, development time from egg hatch to adult, and pupal weight. Methods and results of these studies are described in S2 Appendix.

Helicoverpa zea population abundance and damage association

Year-to-year differences in H. zea population abundance over the study period could account for changes in control efficacy. To test this, we obtained archived blacklight trap data from the Maryland Department of Agriculture, which conducted a statewide monitoring network over the study period up to 2014 [55]. Additional trap data was obtained from the University of Delaware Insect Trapping Program [58] for years 2015 and 2016. Both data sets contained H. zea moth activity from traps at and near our farm locations. We calculated nightly mean moth numbers for each year by averaging across multiple trap sites, over a 14-day period starting at the onset of silking at each planting.

We analysed trends in H. zea population abundance at the sites, and its association with damages for Bt hybrids, through LMMs based on REML. For H. zea abundance, the LMM included mean nightly moth captures as response, year as fixed effect, and study site as random effect to account for repeated measurement. For LMM analysing the relationship between H. zea population abundance and damage in Bt hybrids, damaged corn ears (percentage) for Bt hybrids was treated as the response, mean nightly H. zea abundance as predictor, and site as random variable to account for repeated measures.

Efficacy and tissue toxicity comparisons among the Bt hybrids

The same hybrids of Cry1A.105+Cry2Ab2 sweet corn were evaluated over each study period. However, different Cry1Ab hybrids were planted over the study period as they became commercially available and widely used by growers. Plots were planted with Bt hybrid ‘GSS0937’ and its isoline ‘Bonus’ during 1996–1997, Bt hybrid ‘GSS0966’ and its isoline ‘Prime Plus’ during 1998–2001, and Bt bicolor hybrid ‘BC0805’ and its isoline ‘Providence’ for the remainder years (2002–2014). To explore the possibility that differences in toxin expression among hybrids could account for changes in control efficacy, field performance of six Cry1Ab hybrids and the non-Bt expressing hybrid Providence were evaluated in 2008. Hybrids included BC0805 and GSS0966, along with newer hybrids (BSS0977, BSS0982, WH0809, and WH0812) that were not used in the study. The GSS0937 hybrid planted during the first two years was not included because seed was not available. Five replicate blocks of the seven hybrids (four at Queenstown, one at Upper Marlboro) were planted over a three-week period during June to provide silking stages attractive to a range of H. zea moth pressure during the late summer. To synchronize the silking period among hybrids, plantings in each block were staggered over several days according to the expected maturity time of each hybrid. Plots consisted of four rows spaced 90 cm apart and 15 m long, and were managed according to recommended commercial practices including overhead irrigation but no insecticide applications. Replicate blocks of hybrids were harvested at fresh market maturity on August 22, September 8, 18, and 24, and October 7. Data were recorded (as described above) on the percentage of ears damaged, mean instar stage, and extent of kernels consumed by each insect pest by examining 100 ears per plot.

We compared the rate of damage, instar and consumption among the six Bt hybrids and non-Bt hybrid ‘Providence’ using LMMs based on REML, assuming normal errors. We constructed separate LMMs, each with damage, instar and consumption as response variables, variety as the predictor, and site as a random effect to account for the site level differences. Tukey’s HSD tests (α = 0.05) was used to identify significant differences in the pairwise comparisons of the estimated means.

We further tested for potential differences in Cry1Ab toxicity (possibly due to expression) among the seven hybrids. Tissue samples of fresh green silk, wilted silk (after pollination), brown silk (at harvest), and kernel tissue (at harvest) were collected from the field plots at 2, 7, 18, and 18 days after the onset of silking, respectively. The frozen tissue material was lyophilized and processed into a fine powder in a tissue grinder, and stored at -80°C until further usage. The level of biological activity of Cry1Ab in each tissue type was determined by a diet-incorporated feeding bioassay with neonate H. zea as the sensitive indicator. We obtained susceptible H. zea eggs from a laboratory colony reared over many generations at the U.S. Department of Agriculture—Agricultural Research Service, Corn Insects and Crop Genetics Research Unit in Ames, Iowa. Eggs were incubated in an environmental chamber under temperature regimes manipulated to schedule a supply of test larvae for each replicate bioassay. The powdered tissue type from each hybrid was mixed in a H. zea meridic diet (Southland Products, Lake Village, AR) at a concentration of 3 g per liter of diet, which results in statistically detectable responses of body weight gain with little mortality [44].

Neonate H. zea were reared individually in Bio-Serv 128-cell clear plastic bioassay trays with clear film lid covers, with each cell containing 1.5 ml of diet. The larvae were allowed to feed for seven days, after which data were recorded on the weight and instar stage of surviving larva. The percentage of growth inhibition was calculated based on the difference in body weight relative to the weight of larvae fed on non-expressing tissue of each hybrid. In total, we tested 128 larvae in each of four replicate bioassays of each tissue type, collected from the corresponding replicate field blocks. H. zea body weight, growth inhibition, and instar stage among different Bt hybrids relative to the non-Bt expressing hybrid served as indicators of potential differences in the tissue toxicity.

Differences among Bt hybrids and the non-Bt hybrid for H. zea weight and growth inhibition were analysed by GLM assuming a Gaussian error distribution and identity link function. Tukey’s HSD tests (α = 0.05) identified significant differences in the pairwise comparisons of the GLM estimated means. We used diagnostic plots visualizing within-group residuals (standardized residuals Vs fitted values, normal Q-Q plots, histograms of residuals) and estimated random effects (normal Q-Q plots and pairs-scatter plot matrix) to ensure LMM appropriateness (see [59]; pgs. 174–197). Package ‘lme4’ [60] was used to construct the LMMs / GLMM, multiple comparison contrasts and Tukey’s HSD comparisons were performed with packages “contrast” and “multcomp” [61,62]. Estimated coefficients were extracted from the LMMs and plotted using “ggplot2” [63], all in R program [64].


Control efficacy assessments

Data from Cry1Ab hybrids and the non-Bt counterparts were analysed for H. zea development and ear damage. During all years, H. zea infestations and ear damage were very high in the non-Bt hybrids, averaging 82.4±17.5% damaged ears, with 5.13±2.6 cm2 of kernel area consumed by larvae consisting of 80.3±17.6% late instars. Trends in these responses over years showed either no change or slight increases. Comparing trends between Bt and non-Bt hybrids, LMMs revealed significant interactions between year and hybrid type for all response variables denoting significant slope differences—damage [F (1,175) = 18.7, P < 0.001]; consumption [F (1,167) = 12.6, P <0.001]; instars [F (1,169) = 9.4, P = 0.009] and proportion of late instars [F (1,281) = 94.1, P < 0.001] (model coefficients are available in Table 1 of S3 Appendix). Changes over time in damage, consumption, instars and proportion of late instars were significantly different between Bt and non-Bt hybrids, with steeper increases for Bt than non-Bt hybrids (Fig 1A–1D). Over the 21 years, Cry1Ab hybrids experienced a greater change (88% relative increase) in ear damage by H. zea than non-Bt hybrids (Fig 1A), with 6.3% of the ears damaged in 1996 compared to 85.1% damaged ears in 2016 (based on raw averages). Since 1996, mean area of Bt kernels consumed per ear increased from 0.6 cm2 to about 3 cm2 (Fig 1B), while area of non-Bt hybrid consumption remained about the same or had declined marginally. The mean instar recorded in Bt hybrids also increased over the study period, indicating that surviving larvae reached later developmental stages (Fig 1C), while there was relatively no change for non-Bt hybrids. In particular, the proportion of late instars in Bt hybrids increased markedly over the past decade compared to that of non-Bt hybrids. Relatively few surviving larvae reached the 4th instar in Bt ears during 1996–2006, while 37% of the surviving larvae were 4th-6th instars during 2015–2016 (Fig 1D).

Fig 1. Trends comparing efficacy of Cry1Ab Bt sweet corn (Attribute) with non-Bt isogenic hybrids for control of Helicoverpa zea during 1996–2016 in Maryland, USA.

Over years, Bt hybrids (blue circles and shades) had significant increases in the percentage of H. zea damaged ears (A), kernel consumption (B), instar stage (C) and proportion of late instars (D) than non-Bt hybrids (yellow squares and shades). Points represent the raw data, black lines represent the predictions from LMMs, while shaded region denote the upper and lower confidence levels (95% CI).

Similar trends are evident in Fig 2 showing increasing H. zea infestations and ear damage resulting in reduced field efficacy of the Cry1A.105+Cry2Ab2 sweet corn hybrids. Of the 50 plantings evaluated during 2010–2016, LMMs revealed significant interactions between year and hybrid type for all response variables denoting significant steeper slopes for the Bt hybrids—damage [F (1,93) = 18.9, P < 0.001]; consumption [F (1,90) = 14.4, P <0.001]; instars [F (1,91) = 12.9, P <0.001] and proportion of late instars [X2 = 67.9, P < 0.001] (model coefficients are available in Table 2 of S3 Appendix). Ear damage (mean 87.1±11.2%), kernel consumption (mean 5.5±1.79 cm2) and the proportion of late instars (mean 83.4±12.2%) in the isogenic non-Bt hybrids showed only slight increases or no significant change over the seven years (Fig 2). Damaged ears of Cry1A.105+Cry2Ab2 sweet corn averaged 20.2±12.4% during 2010–2012, with 0.13±0.11 cm2 of kernel area consumed by larvae consisting of only 6.4±8.69% late instars. The field efficacy rapidly changed during 2015–2016 when damaged ears increased to 59.5 ±27.6% and kernel area consumed increased to 2.5±1.9 cm2, with 70.4±17.5% of the surviving H. zea reaching late instars (Fig 2A–2D).

Fig 2. Trends comparing efficacy of Cry1A.105+Cry2Ab2 Bt sweet corn (Performance Series) with non-Bt isogenic hybrids for control of Helicoverpa zea during 2010–2016 in Maryland, USA.

Over years, Bt hybrids (blue circles and shades) had significant increases in the percentage of H. zea damaged ears (A), kernel consumption (B), instar stage (C) and proportion of late instars (D) than non-Bt hybrids (yellow squares and shades). Points represent the raw data, black lines represent the predictions from LMMs / GLMM, while shaded region denote the upper and lower confidence levels (95% CI).

Data from 13 plantings of Vip3A + Cry1Ab sweet corn evaluated during 2008–2016 were not analysed because no live larvae and no ear damage were found. The ears of non-Bt isogenic hybrids, paired with these Bt plots at each planting, experienced high H. zea infestations, resulting in 87.9±14.1% damaged ears and 5.4±2.4 cm2 kernel area consumed. Under this high pressure, the pyramided hybrids expressing Vip3A + Cry1Ab toxins provided 100% control of H. zea, as well as fall armyworm and European corn borer.

Bioassays for resistance characterization

When fed diet without leaf powder, larval weight gain (218.0±19.92 mg) of the susceptible strain was 27% more than that of the UMD 2015 strain (159.1±17.9 mg). Although not significantly different [F (1,3) = 5.57, P = 0.099], this suggests that the susceptible strain may be more adapted to the artificial diet. However, leaf tissue-incorporated bioassay results showed a significant interaction between strain and tissue concentration for weight gain [X2 = 46.27, df = 1, P < 0.001]. Weight gain of the susceptible strain was significantly reduced at a greater rate than the UMD 2015 strain at all concentrations tested (Fig 3).

Fig 3. Comparison of weight between susceptible laboratory and field collected Maryland populations of Helicoverpa zea across concentrations of Cry1Ab expressing green leaf tissue.

At every diet concentration other than control (dosage = 0), weight of larvae (mg) after 1 week of feeding assays was significantly higher for the Maryland strain (blue), than the susceptible (orange) strain. Points represent the raw data values; while the squares represent quasi-Poisson GLM estimated means, and the vertical lines denoting the confidence intervals around the mean. Asterisks indicate statistically significant differences (P < 0.05) based on post-hoc comparisons with a Bonferroni correction.

Helicoverpa zea population abundance and damage association

The population abundance of H. zea during the 14-day period following silking at each planting decreased significantly over the study period from 3 moths captured per night in 1996 to 1.3 in 2014 [F (1, 165) = 48.7, P<0.001; slope = -0.10; Fig 4A]. Additional data from 12 trap locations on the Delmarva Peninsula showed even lower H. zea moth activity, with captures per night averaging 0.64±0.48 in 2015 and 0.42±0.45 in 2016. H. zea population abundance did not significantly affect the observed damages to corn ears for Bt hybrids [F (1, 82) = 0.001, P = 0.97; Fig 4B].

Fig 4. Mean nightly captures of Helicoverpa zea in black light traps during 1996–2014 in Maryland, USA and its association with damage to Bt corn hybrids.

The population abundance of H. zea at or near study sites decreased over the past two decades (A), and showed no relationship with damage levels in Bt sweet corn hybrids (B). Lines represent predictions from LMMs and shades depict upper and lower confidence intervals (95% CI).

Efficacy and tissue toxicity comparisons among the Bt hybrids

The seven hybrids within each replicate block reached the silking stage within several days of each other and thus were exposed similarly to the oviposition pressure by H. zea. High ear infestations in the non-Bt hybrid caused an overall 70% damaged ears and 2.75 cm2 of kernel consumption, and larvae found in ears averaged 4.5 instar stage in developmental growth. Values of damage, consumption, and mean instars across the Bt hybrids were significantly less than the non-Bt control hybrid but did not vary significantly among the Bt hybrids (Fig 5A–5C; see Table 3 in S3 Appendix for statistical tables). The mean weight of larvae feeding on different corn tissues was similar among the Bt hybrids and significantly less than non-Bt control hybrids (Fig 6). Inhibition of larval growth upon feeding on different tissues was also not significantly different among Bt hybrids but significantly higher than the non-Bt hybrid (Fig 6). The mean instar feeding on different sweet corn tissues was also similar among the Bt hybrids, and significantly less than the non-Bt hybrid (Fig 6). Brown dried silk and kernel tissue allowed 46% more weight gain and 4.5% more stadia development than that of green and wilted silk tissue, but there were no differences among the Bt hybrids.

Fig 5. Results comparing control efficacy variables among Bt and non-Bt hybrid varieties in Maryland, USA in 2008.

The mean damaged ears (A), kernel area consumed, (B), and instars of susceptible larvae (C) was broadly similar among the Cry1Ab expressing Bt hybrids (blue bars), and significantly different (Tukey’s HSD; α = 0.05; denoted by unique alphabets) from non-Bt control hybrids (yellow bar). Black lines represent the mean values and the height of bars above and below the black lines respectively indicate the upper and lower confidence levels (95% CI) estimated through LMMs.

Fig 6. Results comparing control efficacy in relation to tissue toxicity among Bt and non-Bt sweet corn varieties from Maryland, USA in 2008.

The mean weight, growth inhibition and instars of susceptible larvae feeding on different sweet corn tissues was broadly similar among the Cry1Ab expressing Bt hybrids (blue bars), and significantly different (Tukey’s HSD; α = 0.05) from non-Bt control hybrids (yellow bar). Black lines represent the mean values and height of bars indicate the upper and lower confidence levels (95%CI) estimated through Gaussian GLMs or ANOVA.


Our field results clearly demonstrate the significantly increased susceptibility and reduced control efficacy of Cry1Ab Bt sweet corn (event Bt11) to H. zea, since its commercial introduction in 1996. We also report significant reductions in field performance of Cry1A.105+Cry2Ab2 sweet corn (event MON89034) for controlling H. zea, particularly during 2015–2016. Larvae successfully infested and damaged an increasingly large proportion of ears, consumed more kernel area, and reached later developmental stages (4th - 6th instars) in both events of Bt hybrids with increasing years of adoption. The control efficacy failure was unrelated to the H. zea population abundance. Moth activity monitored in blacklight traps declined over the past 21 years at the study sites. Among the different Cry1Ab hybrids, there was no evidence of tissue toxicity differences that could contribute to the decline in control efficacy. Field efficacy comparisons under high H. zea population pressure also showed that ear damage, consumption, and mean instars did not differ significantly among Cry1Ab expressing hybrids. Similarly, bioassay determinations of various plant tissues did not show significant Bt hybrid differences in H. zea body weight gains, percentage growth inhibition, or developmental larval stage. After ruling out these possible contributing factors, the rapid change in field efficacy in recent years and decreased susceptibility of H. zea to Bt sweet corn provide strong evidence of field-evolved resistance in H. zea populations to multiple Cry toxins. However, our field studies on Vip3A + Cry1Ab sweet corn (Attribute II) show no detectable change in H. zea susceptibility and confirm the high efficacy of this pyramided product reported earlier [50]. Our field results for Vip3A hybrids suggest that there may be no cross resistance with Cry1Ab, similar to previous reports of no cross-resistance for Vip3A with laboratory colonies of Cry1Ac resistant H. zea [38,39].

Results of our laboratory bioassays further demonstrate significant differences in weight gain and fitness characteristics between the susceptible strain and the UMD 2015 strain of H. zea reared from surviving late instars collected from Cry1Ab sweet corn. Although apparently more adapted to the artificial diet, weight gain of the susceptible strain significantly reduced at a greater rate than the UMD 2015 strain at all concentrations tested. Using Cry1Ab-expressing corn leaf powder Anilkumar et al. [38] showed significant, but marginal differences in weight loss (no differences in mortality) between susceptible and Cry1Ac-resistant H. zea. Fitness of the UMD 2015 strain was significantly lower than that of the susceptible strain as indicated by lower hatch rate, longer time to adult eclosion, lower pupal weight, and reduced survival to adulthood (see S2 Appendix). These results suggest that reduced fitness in the UMD 2015 strain is likely associated with changes in susceptibility to Cry toxins, which has been reported in other insects associated with resistance to Bt [27,65].

The fitness costs may also have broadly affected the timeframe of resistance evolution as well as the stability of resistance in the field. Previous reports identify sub-lethal effects of MON810 corn resulting in prolonged larval and pupal development, delayed adult eclosion and emergence, thereby resulting in asynchrony of mating between H. zea individuals [49,66]. Reports indicate that longer larval developmental period in resistant S. frugiperda has resulted in emergence asynchrony between adults susceptible and resistant to Cry1F (Bt maize event TC1507) in Puerto Rico [67]. Similarly, the prolonged larval and pupal development and later emergence of resistant adults (than susceptible strains) and resultant asynchrony in emergence and mating between resistant and susceptible strains could have delayed field-evolved resistance to Cry proteins in H. zea. Additionally, other fitness costs may have made it difficult for the resistant Maryland population to increase significantly to cause widespread field control failure earlier. Our previous unsuccessful three attempts at characterizing resistance evolution (see S1 Appendix) may be attributed to fitness costs associated with resistance development.

The field-evolved resistance we report here indicate ‘practical resistance’ (>50% resistant individuals and reduced efficacy [16,18]) given the probable genetic basis of resistance. Many sweet corn farmers in Maryland either have stopped growing Cry1Ab hybrids or are applying more insecticide sprays to compensate for the reduced control efficacy (personal communication, GPD). In 2016, there also have been numerous inquiries to seed companies from sweet corn farmers reporting control failures from Cry1A.105+Cry2Ab2 hybrids (personal communication, GPD). Our results confirm the findings from recent studies by Reisig and Reay-Jones [68,69] showing increases in kernel feeding by H. zea on Cry1A.105+Cry2Ab2 field corn (VT Double PRO) and evidence of developing resistance to the Cry1Ab trait based on changes over time in toxin inhibition on growth and development of H. zea.

Many factors could have contributed to development of H. zea resistance. The Cry1Ab toxin has been exerting selection pressure on H. zea populations in Bt corn since the trait became commercially available in 1996; however, we presume that the relatively low deployment of Bt sweet corn hybrids, planted without a refuge requirement, has unlikely exerted enough selection pressure alone to account for changes in H. zea susceptibility. Instead, the high adoption rate of Bt field corn and cotton, along with the moderate dose expression of Cry1Ab and related Cry1A toxins in these crops and decreasing refuge compliance, probably contributed significantly for evolution of resistance. Many field corn hybrids expressing Cry1Ab (events MON810 and BT11) or Cry1A.105+Cry2Ab2 (event MON89034) are widely used and the moderate dose expression could allow heterozygous resistant individuals containing minor resistance alleles to survive, thus increasing the frequency of genes that confer resistance in the H. zea population [13,70]. Regional deployment levels of Bt corn hybrids can also contribute to increasing resistant gene frequencies, with low technology adoption related to slower rate of resistance evolution [71]. The adoption rate of Bt field corn in Maryland is very high, accounting for 83–93% of the hectares planted during 2013 in crop reporting districts where the Queenstown and Salisbury sites are located. This high adoption of Bt corn, along with a presumed decline in compliance with the refuge requirements, has almost certainly contributed at the local level to the evolution of resistance. Similarly, Bt corn adoption exceeds 80% throughout most corn production areas in the U.S., and surveys show that 22% of the farmers are not complying with refuge requirements [72].

The behavior and life history characteristics of H. zea may have aided in evolution of resistance, similar to documented cases of evolution of resistance to conventional insecticides [7375]. At eastern Maryland sites, H. zea overwinters successfully during most years and thus resistant individuals are able to contribute resistant alleles to the population in the subsequent year. In addition to local recruitment of resistant H. zea individuals, southerly flow weather patterns can facilitate the northward dispersal of moths, particularly as the maturing crops in the southern regions become less attractive as hosts [76]. This south-north migration of moths already selected for resistance on Bt corn and cotton can enhance the development of Cry1Ab resistance in the northern corn growing regions. Reisig and Reay-Jones [68] recently presented evidence of developing resistance to the Cry1Ab trait in field corn in the South and North Carolinas.

Behavioral changes in H. zea due to feeding on Bt corn can also increase the risk of evolution of resistance. Studies in Maryland reported that sublethal exposure to Cry1Ab toxin in Bt corn delayed larval development and adult emergence, which may result in asynchrony of mating between individuals emerging from Bt and non-Bt corn [66]. Another study showed that alterations in the cannibalistic behavior of H. zea larvae due to sublethal exposure to the Cry1Ab toxin could increase the selective differential between susceptible individuals and those carrying resistance genes [77]. The extent that each behavioral factor contributes to the current field efficacy failures and H. zea resistance to Cry1Ab is unknown, but collectively they probably have aided in the evolution of resistance.

The field-evolved resistance by H. zea has implications for resistance monitoring, IRM and the sustainability of the Bt corn technology. Registrants of Bt field corn expressing Cry1Ab, and Cry1A + Cry2Ab2 toxins are required by EPA to annually monitor populations of H. zea using laboratory bioassays to detect field-evolved resistance early enough to enable proactive management before field failures occur [43]. Maryland has historically represented the northern range of overwintering H. zea [54]. With these populations evolving resistance, programs monitoring for resistance in further northern ranges of H. zea are essential. Warming temperatures exacerbate the risk of resistance spreading, as latitudes north of 40° become conducive for successful overwintering and increasing migration of H. zea [15,78].

We predict that H. zea resistance to the Cry toxins is likely to increase, and spread, with the shift to RIB corn hybrids that contain a blend (e.g. 95:5 Bt: non-Bt seed). Similarly, due to northward influxes of potentially resistant moths from southern source regions, the risk of further evolution of resistance may increase with the reduced refuge size (from 50% to 20%) in regions where Bt cotton is used. Apart from reductions in the refuge size, there are also concerns that pollen-mediated gene flow between Bt and refuge plants in a seed blend could accelerate resistance evolution. Cross-pollination between refuge and neighboring Bt plants can result in fewer susceptible H. zea moths produced in a refuge or intermediate levels of toxin expressed in kernels that kill susceptible individuals but allow heterozygotes to survive [79,80]. The potential existence of cross-resistance between Cry1Ab and the other Cry toxins [13,35,39,8183] may also compromise the efficacy and durability of the new pyramided traits in Bt field and sweet corn. Finally, as reported here and by Burkness et al. [50], Vip3A expression in Attribute II sweet corn and many field corn products is still highly effective for controlling H. zea and other lepidopteran pests. Although there is no reported cross-resistance between Vip3A and Cry toxins [38,81,84], it is unknown whether continued selection pressure from Cry expressing Bt corn and increased use of the Viptera trait will reduce the sustainability of this pyramided Bt technology.

Supporting Information

S1 Appendix. Experiments to characterize Bt resistance in Helicoverpa zea field-collected populations during 2008 to 2012.


S2 Appendix. 2015 Bioassays to characterize fitness of Maryland field-collected populations of Helicoverpa zea.


S3 Appendix. Tables presenting the summary of statistical results for all analyses.



We thank the research farm managers, David Armentrout, Mike Newell, Alfred Hawkins, Kevin Conover, and Dave Justice for establishing and maintaining the paired plantings of Bt and non-Bt sweet corn. We particularly thank William Moar (Auburn University), Bruce Lang (Custom BioProducts), Phillip Matthews (Syngenta), and Ryan Kurtz (formally with Syngenta) for their efforts in establishing laboratory colonies to characterize Cry1Ab resistance. We greatly appreciate Mike Embry, Terry Patton, Amy Miller, the many research assistants, summer student interns, graduate students, and technicians over the past 21 years for their help with data collection and field collection of surviving larvae. Finally, we thank Doug Plaisted, Debbie Warnick, and others from Syngenta Seeds for providing sweet corn seed and technical assistance. Comments from three anonymous reviewers and Carlos Blanco improved the manuscript.

This publication was developed under Assistance Agreement No. X3-83588701 awarded by the United States Environmental Protection Agency (U.S. EPA) to the American Association for the Advancement of Science (AAAS). It has not been formally reviewed by the U.S. EPA. The views expressed in this document are solely those of the authors, and do not reflect those of either U.S. EPA or AAAS. Products or commercial services mentioned in this publication are solely for reference purposes only, and do not represent endorsement by the authors, the U.S. EPA, or AAAS.

Author Contributions

  1. Conceptualization: GPD.
  2. Data curation: GPD PDV.
  3. Formal analysis: GPD PDV.
  4. Funding acquisition: GPD CF.
  5. Investigation: GPD PDV CF.
  6. Methodology: GPD PDV CF.
  7. Project administration: GPD CF.
  8. Resources: GPD PDV CF.
  9. Supervision: GPD.
  10. Validation: GPD CF.
  11. Visualization: PDV.
  12. Writing – original draft: PDV GPD.
  13. Writing – review & editing: PDV GPD CF.


  1. 1. James C. Global status of commercialized biotech/GM crops [Internet]. Ithaca, New York: International Service for the Acquisition of Agri-biotech Applications; 2014. Report No.: ISAAA Brief No. 49.
  2. 2. Pray CE, Huang J, Hu R, Rozelle S. Five years of Bt cotton in China—the benefits continue. Plant J. 2002;31: 423–430. pmid:12182701
  3. 3. Wu K-M, Lu Y-H, Feng H-Q, Jiang Y-Y, Zhao J-Z. Suppression of cotton bollworm in multiple crops in China in areas with Bt toxin—containing cotton. Science. 2008;321: 1676–1678. pmid:18801998
  4. 4. Hutchison WD, Burkness EC, Mitchell PD, Moon RD, Leslie TW, Fleischer SJ, et al. Areawide suppression of European corn borer with Bt maize reaps savings to non-Bt maize growers. Science. 2010;330: 222–225. pmid:20929774
  5. 5. National Research Council. The impact of genetically engineered crops on farm sustainability in the United States. Washington D.C.: The National Academic Press; 2010.
  6. 6. Kathage J, Qaim M. Economic impacts and impact dynamics of Bt (Bacillus thuringiensis) cotton in India. Proc Natl Acad Sci. 2012;109: 11652–11656. pmid:22753493
  7. 7. Qaim M, Kouser S. Genetically modified crops and food security. PLoS ONE. 2013;8: e64879. pmid:23755155
  8. 8. Klümper W, Qaim M. A meta-analysis of the impacts of genetically modified crops. PLoS ONE. 2014;9: e111629. pmid:25365303
  9. 9. National Academies of Sciences, Engineering & Medicine. Genetically engineered crops: experiences and prospects [Internet]. The National Academies Press; 2016.
  10. 10. U. S. Department of Agriculture—National Agricultural Statistics Service. USDA/NASS QuickStats [Internet]. 2015 [cited 13 Aug 2015].
  11. 11. U. S. Department of Agriculture—Economic Research Service. Recent trends in GE adoption [Internet]. 2015 [cited 27 Jul 2015].
  12. 12. Matten SR, Frederick RJ, Reynolds AH. United States Environmental Protection Agency insect resistance management programs for plant-incorporated protectants and use of simulation modeling. In: Wozniak CA, McHughen A, editors. Regulation of agricultural biotechnology: the United States and Canada. Springer Netherlands; 2012. pp. 175–267.
  13. 13. Gould F. Sustainability of transgenic insecticidal cultivars: integrating pest genetics and ecology. Annu Rev Entomol. 1998;43: 701–726. pmid:15012402
  14. 14. US EPA. Insect resistance management fact sheet for Bacillus thuringiensis (Bt) corn products. Office of Pesticide Programs [Internet]. 3 Feb 2014 [cited 3 Jul 2015].
  15. 15. Olmstead DL, Nault BA, Shelton AM. Biology, ecology, and evolving management of Helicoverpa zea (Lepidoptera: Noctuidae) in sweet corn in the United States. J Econ Entomol. 2016; tow125.
  16. 16. Tabashnik BE, Brévault T, Carrière Y. Insect resistance to Bt crops: lessons from the first billion acres. Nat Biotechnol. 2013;31: 510–521. pmid:23752438
  17. 17. Tabashnik BE. ABCs of insect resistance to Bt. PLOS Genet. 2015;11: e1005646. pmid:26583776
  18. 18. Tabashnik BE, Mota-Sanchez D, Whalon ME, Hollingworth RM, Carrière Y. Defining terms for proactive management of resistance to Bt crops and pesticides. J Econ Entomol. 2014;107: 496–507. pmid:24772527
  19. 19. Storer NP, Babcock JM, Schlenz M, Meade T, Thompson GD, Bing JW, et al. Discovery and characterization of field resistance to Bt maize: Spodoptera frugiperda (Lepidoptera: Noctuidae) in Puerto Rico. J Econ Entomol. 2010;103: 1031–1038. pmid:20857709
  20. 20. Storer NP, Kubiszak ME, Ed King J, Thompson GD, Santos AC. Status of resistance to Bt maize in Spodoptera frugiperda: lessons from Puerto Rico. J Invertebr Pathol. 2012;110: 294–300. pmid:22537834
  21. 21. Farias JR, Andow DA, Horikoshi RJ, Sorgatto RJ, Fresia P, dos Santos AC, et al. Field-evolved resistance to Cry1F maize by Spodoptera frugiperda (Lepidoptera: Noctuidae) in Brazil. Crop Prot. 2014;64: 150–158.
  22. 22. Huang F, Qureshi JA, M RL Jr, Reisig DD, Head GP, Andow DA, et al. Cry1F resistance in fall armyworm Spodoptera frugiperda: single gene versus pyramided Bt maize. PLOS ONE. 2014;9: e112958. pmid:25401494
  23. 23. Monnerat R, Martins E, Macedo C, Queiroz P, Praça L, Soares CM, et al. Evidence of field-evolved resistance of Spodoptera frugiperda to Bt corn expressing Cry1F in Brazil that is still sensitive to modified Bt toxins. PLoS ONE. 2015;10: e0119544. pmid:25830928
  24. 24. Omoto C, Bernardi O, Salmeron E, Sorgatto RJ, Dourado PM, Crivellari A, et al. Field-evolved resistance to Cry1Ab maize by Spodoptera frugiperda in Brazil. Pest Manag Sci. 2016; n/a–n/a.
  25. 25. van Rensburg JBJ. First report of field resistance by the stem borer, Busseola fusca (Fuller) to Bt-transgenic maize. South Afr J Plant Soil. 2007;24: 147–151.
  26. 26. Dhurua S, Gujar GT. Field-evolved resistance to Bt toxin Cry1Ac in the pink bollworm, Pectinophora gossypiella (Saunders) (Lepidoptera: Gelechiidae), from India. Pest Manag Sci. 2011;67: 898–903. pmid:21438121
  27. 27. Gassmann AJ, Petzold-Maxwell JL, Keweshan RS, Dunbar MW. Field-evolved resistance to Bt maize by western corn rootworm. PLoS ONE. 2011;6: e22629. pmid:21829470
  28. 28. Gassmann AJ. Field-evolved resistance to Bt maize by western corn rootworm: Predictions from the laboratory and effects in the field. J Invertebr Pathol. 2012;110: 287–293. pmid:22537837
  29. 29. Gassmann AJ, Petzold-Maxwell JL, Clifton EH, Dunbar MW, Hoffmann AM, Ingber DA, et al. Field-evolved resistance by western corn rootworm to multiple Bacillus thuringiensis toxins in transgenic maize. Proc Natl Acad Sci. 2014;111: 5141–5146. pmid:24639498
  30. 30. Tabashnik BE, Gassmann AJ, Crowder DW, Carriére Y. Insect resistance to Bt crops: evidence versus theory. Nat Biotechnol. 2008;26: 199–202. pmid:18259177
  31. 31. Moar W, Roush R, Shelton A, Ferré J, MacIntosh S, Leonard BR, et al. Field-evolved resistance to Bt toxins. Nat Biotechnol. 2008;26: 1072–1074. pmid:18846068
  32. 32. Tabashnik BE, Gassmann AJ, Crowder DW, Carrière Y. Response to: Field-evolved resistance to Bt toxins. Nat Biotechnol. 2008;26: 1074–1076.
  33. 33. Reisig D, Reay-Jones FPF. Inhibition of Helicoverpa zea (Lepidoptera: Noctuidae) growth by transgenic corn expressing bt toxins and development of resistance to Cry1Ab. Environ Entomol. 2015;44: 1275–1285. pmid:26314074
  34. 34. Tabashnik BE, Unnithan GC, Masson L, Crowder DW, Li X, Carrière Y. Asymmetrical cross-resistance between Bacillus thuringiensis toxins Cry1Ac and Cry2Ab in pink bollworm. Proc Natl Acad Sci. 2009;106: 11889–11894. pmid:19581574
  35. 35. Brévault T, Heuberger S, Zhang M, Ellers-Kirk C, Ni X, Masson L, et al. Potential shortfall of pyramided transgenic cotton for insect resistance management. Proc Natl Acad Sci. 2013;110: 5806–5811. pmid:23530245
  36. 36. Bernardi D, Salmeron E, Horikoshi RJ, Bernardi O, Dourado PM, Carvalho RA, et al. Cross-resistance between Cry1 proteins in fall armyworm (Spodoptera frugiperda) may affect the durability of current pyramided bt maize hybrids in Brazil. PLOS ONE. 2015;10: e0140130. pmid:26473961
  37. 37. Wei J, Guo Y, Liang G, Wu K, Zhang J, Tabashnik BE, et al. Cross-resistance and interactions between Bt toxins Cry1Ac and Cry2Ab against the cotton bollworm. Sci Rep. 2015;5: 7714. pmid:25586723
  38. 38. Anilkumar KJ, Rodrigo-Simón A, Ferré J, Pusztai-Carey M, Sivasupramaniam S, Moar WJ. Production and characterization of Bacillus thuringiensis Cry1Ac-Resistant Cotton Bollworm Helicoverpa zea (Boddie). Appl Environ Microbiol. 2008;74: 462–469. pmid:18024681
  39. 39. Welch KL, Unnithan GC, Degain BA, Wei J, Zhang J, Li X, et al. Cross-resistance to toxins used in pyramided Bt crops and resistance to Bt sprays in Helicoverpa zea. J Invertebr Pathol. 2015;132: 149–156. pmid:26458274
  40. 40. Santos-Amaya OF, Rodrigues JVC, Souza TC, Tavares CS, Campos SO, Guedes RNC, et al. Resistance to dual-gene Bt maize in Spodoptera frugiperda: selection, inheritance, and cross-resistance to other transgenic events. Sci Rep. 2015;5: 18243. pmid:26675246
  41. 41. Yang F, Kerns DL, Brown S, Kurtz R, Dennehy T, Braxton B, et al. Performance and cross-crop resistance of Cry1F-maize selected Spodoptera frugiperda on transgenic Bt cotton: implications for resistance management. Sci Rep. 2016;6: 28059. pmid:27301612
  42. 42. Hernández-Rodríguez CS, Hernández-Martínez P, Rie JV, Escriche B, Ferré J. Shared midgut binding sites for Cry1A.105, Cry1Aa, Cry1Ab, Cry1Ac and Cry1Fa proteins from Bacillus thuringiensis in two important corn pests, Ostrinia nubilalis and Spodoptera frugiperda. PLOS ONE. 2013;8: e68164. pmid:23861865
  43. 43. Tabashnik BE, Rensburg JBJV, Carrière Y. Field-evolved insect resistance to Bt crops: definition, theory, and data. J Econ Entomol. 2009;102: 2011–2025. pmid:20069826
  44. 44. Siegfried BD, Spencer T, Nearman J. Baseline susceptibility of the corn earworm (Lepidoptera: Noctuidae) to the Cry1Ab toxin from Bacillus thuringiensis. J Econ Entomol. 2000;93: 1265–1268. pmid:10985041
  45. 45. Siegfried BD, Spencer T, Crespo AL, Storer NP, Head GP, Owens E, et al. Ten years of Bt resistance monitoring in the European corn borer: what we know, what we don’t know, and what we can do better. Am Entomol. 2007;53: 208–214.
  46. 46. Marçon PCRG, Young LJ, Steffey KL, Siegfried BD. Baseline susceptibility of European corn borer (Lepidoptera: Crambidae) to Bacillus thuringiensis toxins. J Econ Entomol. 1999;92: 279–285.
  47. 47. Venette RC, Hutchison WD, Andow DA. An in-field screen for early detection and monitoring of insect resistance to Bacillus thuringiensis in transgenic crops. J Econ Entomol. 2000;93: 1055–1064. pmid:10985012
  48. 48. Storer NP, Duyn JWV, Kennedy GG. Life history traits of Helicoverpa zea (Lepidoptera: Noctuidae) on non-Bt and Bt transgenic corn hybrids in eastern North Carolina. J Econ Entomol. 2001;94: 1268–1279. pmid:11681693
  49. 49. Horner TA, Dively GP, Herbert DA. Development, survival and fitness performance of Helicoverpa zea (Lepidoptera: Noctuidae) in MON810 Bt field corn. J Econ Entomol. 2003;96: 914–924. pmid:12852636
  50. 50. Burkness EC, Dively G, Patton T, Morey AC, Hutchison WD. Novel Vip3A Bacillus thuringiensis (Bt) maize approaches high-dose efficacy against Helicoverpa zea (Lepidoptera: Noctuidae) under field conditions: Implications for resistance management. GM Crops. 2010;1: 337–343. pmid:21844691
  51. 51. Shelton AM, Olmstead DL, Burkness EC, Hutchison WD, Dively G, Welty C, et al. Multi-state trials of Bt sweet corn varieties for control of the corn earworm (Lepidoptera: Noctuidae). J Econ Entomol. 2013;106: 2151–2159. pmid:24224259
  52. 52. Lynch RE, Wiseman BR, Plaisted D, Warnick D. Evaluation of transgenic sweet corn hybrids expressing CryIA(b) toxin for resistance to corn earworm and fall armyworm (Lepidoptera: Noctuidae). J Econ Entomol. 1999;92: 246–252. pmid:10036986
  53. 53. Lynch RE, Wiseman BR, Sumner HR, Plaisted D, Warnick D. Management of corn earworm and fall armyworm (Lepidoptera: Noctuidae) injury on a sweet corn hybrid expressing a cryIA(b) gene. J Econ Entomol. 1999;92: 1217–1222.
  54. 54. Ditman LP, Cory EN. The corn earworm: biology and control. Bull Md Agric Exp Stn. 1931; 443–482.
  55. 55. Dively GP. Insect pests of sweet corn I & II. In: Dively GP, Whalen J, Linduska J, Patton T, Bean D, editors. Vegetable pest management—Pest identification and biology, scouting procedures and recommended actions. Second. Maryland Cooperative Extension Service & Delaware Cooperative Extension Service; 1993. pp. 10–13.
  56. 56. Bolker BM, Brooks ME, Clark CJ, Geange SW, Poulsen JR, Stevens MHH, et al. Generalized linear mixed models: a practical guide for ecology and evolution. Trends Ecol Evol. 2009;24: 127–135. pmid:19185386
  57. 57. Dulmage HT, Boening OP, Rehnborg CS, Hansen GD. A proposed standardized bioassay for formulations of Bacillus thuringiensis based on the international unit. J Invertebr Pathol. 1971;18: 240–245. pmid:4937299
  58. 58. University of Delaware, College of Agriculture and Natural Resources, Cooperative Extension, Insect Trapping Program. In: Delaware historical trap catch [Internet]. [cited 24 Oct 2016].
  59. 59. Pinheiro JC, Bates DM. Mixed effects models in S and S-Plus. New York: Springer; 2000.
  60. 60. Bates D, Maechler M, Bolker B, Walker S. lme4: Linear mixed-effects models using Eigen and S4. R package version 1.1–7. [Internet]. 2014.
  61. 61. Hothorn T, Bretz F, Westfall P. Simultaneous inference in general parametric models. Biom J. 2008;50: 346–363. pmid:18481363
  62. 62. Kuhn M, Weston S, Wing J, Thaler JF and T. contrast: A collection of contrast methods. R package version 0.19. [Internet]. 2013.
  63. 63. Wickham H. ggplot2: elegant graphics for data analysis. [Internet]. New York: Springer; 2009.
  64. 64. R Development Core Team. R: A language and environment for statistical computing. The R foundation for statistical computing, Vienna, Austria [Internet]. 2014.
  65. 65. Gassmann AJ, Carrière Y, Tabashnik BE. Fitness costs of insect resistance to Bacillus thuringiensis. Annu Rev Entomol. 2009;54: 147–163. pmid:19067630
  66. 66. Horner TA, Dively GP, Herbert DA. Effects of MON810 Bt field corn on adult emergence of Helicoverpa zea (Lepidoptera: Noctuidae). J Econ Entomol. 2003;96: 925–930. pmid:12852637
  67. 67. Jakka SRK, Knight VR, Jurat-Fuentes JL. Fitness costs associated with field-evolved resistance to Bt maize in Spodoptera frugiperda (Lepidoptera: Noctuidae). J Econ Entomol. 2014;107: 342–351. pmid:24665719
  68. 68. Reisig DD, Reay-Jones FPF. Inhibition of Helicoverpa zea (Lepidoptera: Noctuidae) growth by transgenic corn expressing Bt toxins and development of resistance to Cry1Ab. Environ Entomol. 2015;44: 1275–1285. pmid:26314074
  69. 69. Reisig D. Earworms/Bollworms in Bt Corn | North Carolina Cooperative Extension [Internet]. 2016 [cited 24 Oct 2016].
  70. 70. Onstad DW, Gould F. Modeling the dynamics of adaptation to transgenic maize by European corn borer (Lepidoptera: Pyralidae). J Econ Entomol. 1998;91: 585–593.
  71. 71. Storer NP, Peck SL, Gould F, Duyn JWV, Kennedy GG. Spatial processes in the evolution of resistance in Helicoverpa zea (Lepidoptera: Noctuidae) to Bt transgenic corn and cotton in a mixed agroecosystem: a biology-rich stochastic simulation model. J Econ Entomol. 2003;96: 156–172. pmid:12650359
  72. 72. Jaffe G. Complacency on the farm: Significant noncompliance with EPA’s refuge requirements threatens the future effectiveness of genetically engineered pest-protected corn [Internet]. Washington D.C.: Center for Science in the Public Interest; 2009 p. 19.
  73. 73. Stadelbacher EA, Snodgrass GL, Elzen GW. Resistance to cypermethrin in first generation adult bollworm and tobacco budworm (Lepidoptera: Noctuidae) populations collected as larvae on wild geranium, and in the second and third larval generations. J Econ Entomol. 1990;83: 1207–1210.
  74. 74. McCaffery AR. Resistance to insecticides in Heliothine Lepidoptera: a global view. Philos Trans R Soc Lond B Biol Sci. 1998;353: 1735–1750.
  75. 75. Jacobson A, Foster R, Krupke C, Hutchison W, Pittendrigh B, Weinzierl R. Resistance to pyrethroid insecticides in Helicoverpa zea (Lepidoptera: Noctuidae) in Indiana and Illinois. J Econ Entomol. 2009;102: 2289–2295. pmid:20069859
  76. 76. Sandstrom M A, Changnon D. Improving our understanding of Helicoverpa zea migration in the midwest: assessment of source populations. Plant Health Prog. 2007;
  77. 77. Horner TA, Dively GP. Effect of MON810 Bt field corn on Helicoverpa zea (Lepidoptera: Noctuidae) cannibalism and its implications to resistance development. J Econ Entomol. 2003;96: 931–934. pmid:12852638
  78. 78. Diffenbaugh NS, Krupke CH, White MA, Alexander CE. Global warming presents new challenges for maize pest management. Environ Res Lett. 2008;3: 044007.
  79. 79. Burkness EC, Hutchison WD. Bt pollen dispersal and Bt kernel mosaics: integrity of non-Bt refugia for Lepidopteran resistance management in maize. J Econ Entomol. 2012;105: 1773–1780. pmid:23156176
  80. 80. Chilcutt CF, Tabashnik BE. Contamination of refuges by Bacillus thuringiensis toxin genes from transgenic maize. Proc Natl Acad Sci U S A. 2004;101: 7526–7529. pmid:15136739
  81. 81. Carrière Y, Crickmore N, Tabashnik BE. Optimizing pyramided transgenic Bt crops for sustainable pest management. Nat Biotechnol. 2015;33: 161–168. pmid:25599179
  82. 82. Yang F, Kerns DL, Head GP, Leonard BR, Levy R, Niu Y, et al. A challenge for the seed mixture refuge strategy in Bt maize: impact of cross-pollination on an ear-feeding pest, corn earworm. PLOS ONE. 2014;9: e112962. pmid:25409442
  83. 83. Brévault T, Tabashnik BE, Carrière Y. A seed mixture increases dominance of resistance to Bt cotton in Helicoverpa zea. Sci Rep. 2015;5: 9807. pmid:25950459
  84. 84. Kurtz RW, McCaffery A, O’Reilly D. Insect resistance management for Syngenta’s VipCot transgenic cotton. J Invertebr Pathol. 2007;95: 227–230. pmid:17475274