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RNAi-Mediated Knockdown of CYP321A7 and CYP321A8 in Fall Armyworm Spodoptera frugiperda (J.E. Smith, 1797) (Lepidoptera: Noctuidae) Enhances Susceptibility to Chlorantraniliprole and Thiamethoxam

Submitted:

20 September 2024

Posted:

21 September 2024

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Abstract
Fall armyworm (FAW), Spodoptera frugiperda, has been causing significant crop losses and has now become the most economically important pest of corn globally. With the challenges arising from the extensive use of synthetic chemicals such as reports that FAW gained resistance to various insecticides, researchers are developing environmentally sound control measures to address these issues. An example is the application of the RNA interference in managing FAW populations. RNA interference is a biological process where dsRNA molecules silence specific gene of interest. Here, dsRNA fragments were generated to target Cytochrome P450 monooxygenases CYP321A7 and CYP321A8 in FAW. Mortality and phenotypic effects of RNAi-mediated knockdown of essential genes of target CYP450s through RNAi in FAW were analyzed. Results showed that RNA in vitro transcription yielded ~14 μg/μL of dsCYP321A7 and dsCYP321A8. The mortality rate of dsCYP321A7- and dsCYP321A8-fed larvae following exposure to insecticide with dual active ingredient of Chlorantraniliprole and Thiamethoxam increased by 90% and 80%, respectively as compared to dsGFP-fed larvae with 40% at 2 days post insecticide exposure. This study provided evidence for the potential of RNAi for FAW management strategies particularly for insecticide-resistant populations, including the potential for biopesticide development.
Keywords: 
Cytochrome P450
;  
dsRNA
;  
RNAi
;  
Spodoptera frugiperda
Subject: 
Biology and Life Sciences  -   Agricultural Science and Agronomy

Introduction

Fall Armyworm (FAW), Spodoptera frugiperda, is a lepidopteran pest that attacks more than 350 plant species in vast numbers, causing significant yield losses if left uncontrolled on cotton, other vegetable crops, and maize, as well as economically significant farmed grasses including sorghum, rice, sugarcane, and wheat (Nwanze et al., 2021). FAW is an invasive pest that originates in America and has spread in Africa in 2018, India (2018-2019) and eventually expanded in Asia-Pacific countries including China, Korea, Japan, Australia and Southeast Asian countries (Navasero, et al., 2020; Yang, et al., 2021a; Kumar, et al., 2022). This agricultural pest is highly polyphagous and mostly feeds on foliage consuming the leaf tissue from one side and leaving the opposite epidermal layer intact (Capinera, 2020).
Significant corn yield losses were reported to different countries that were affected by FAW (Omwoyo, et al., 2022; Kumar, et al., 2022). In Africa, it has a potential to cause corn losses from 8.3 to 20.6 million tons each year if left uncontrolled (Day, et al., 2017). Generally, to control FAW, farmers are using resistant cultivars, insecticides, cultural practices, and integrated pest management approaches (Matova, et al., 2020). However, there are limitations on the success of any of these strategies in providing efficient control in large-scale fields due to high pest pressure (Li, Wang, & Romeis, 2021). Currently, using synthetic insecticides remains to be the primary control of this agricultural pest. Commonly, emamectin benzoate, Bacillus thuringiensis, lambda cyhalothrin, indoxacarb, chlorpyrifos and chlorantraniliprole are used to control FAW (USAid, 2018; Phambala, et al., 2020; Hasnain, et al., 2023). In consequence, the long-term use of these synthetic insecticides could lead to resistant strains (Hafeez, et al., 2022).
Sustainable pest management is continually challenged with insect resistance to synthetic insecticides (Hafeez, et al., 2022). Developing pesticide resistance management techniques requires a thorough understanding of the mechanisms through which insects acquire resistance to insecticides. Mechanism of insecticide resistance includes behavioral, biological, penetration, target-site alteration, metabolic, and resistance-inducing operational factors (Siddiqui et al., 2023). The most common type of insecticide metabolic resistance is monooxygenase-mediated resistance (Scott, 1999). Particularly, Cytochrome P450 monooxygenases (CYP450) are implicated in the metabolism of a broad spectrum of insecticides, facilitating their breakdown or modification into less toxic forms (Ye et al., 2022) through a catalytic cycle involving substrate binding, electron transfer, oxygen activation, oxidation reactions, and product release (Guengerich, 2018). This results in reduced susceptibility of pests to insecticides, necessitating the development of alternative strategies for effective pest control (Siddiqui et al., 2023).
Several studies show that CYP450 genes are highly involved in resistance developments in FAW to various insecticides (Berge et al., 1998). Hafeez et al, (2019) revealed that CY3217A7 and CYP6AE43 were significantly higher mRNA transcript levels in the midgut of FAW population exposed with indoxacarb compared to unexposed population. (Bai-Zhong et al. (2020) also discussed that CYP321A8, CYP321A9, and CYP321B1 were overexpressed in the midgut of second instar FAW larvae after exposure to chlorantraniliprole. Actin was also observed to have stable expression after exposed to an insecticide, emamectin benzoate (Zhou et al., 2021).
Repeated use of chemicals would increase the risk of insect resistance to chemicals. Thus, the demand to innovate approaches in controlling pests is highly encouraged. Using RNA interference (RNAi) would open new avenues for FAW management. Double-stranded RNAi is used to silence gene expression of an organism triggered by a double-stranded RNA (dsRNA) at a cellular level (Agrawal, et al., 2003; Hafeez, et al., 2022). It is a conserved regulatory method known that is used to modulate gene expression in a controlled manner while inducing sequence-specific gene silence (Yao, et al., 2022). A particularly noteworthy feature of RNAi is that the dsRNA is not only capable of entering gut cells but can move to other organs as well in order to produce systemic RNAi in these highly susceptible insects (Joga, et al., 2016). With this, scientists have used this technology to reduce the insect’s susceptibility to insecticides by targeting the CYP450. Laboratory studies have showed successful silencing of target CYP genes to increase the insect’s susceptibility to various insecticides (Hafeez et al., 2022; Nitnavare et al., 2021; Saberi et al., 2024; Y. Zhang et al., 2019). In fact, GreenLight’s Calantha with active ingredient of Ledprona, the first sprayable biopesticide product based on dsRNA, was developed to combat the Colorado Potato Beetle (Rodrigues et al., 2021) and had already granted a registration from US EPA (ID: EPA-HQ-OPP-2021-0271-0194).
This study’s main goal is to develop and evaluate the efficacy of dsRNA for RNA interference (RNAi) to knockdown cytochrome P450 expression in Fall Armyworm, with the aim of contributing a sustainable solution for pest management. Specifically, analyze the mortality and phenotypic effects of knockdown of essential genes of CYP321A7 and CYP321A8.

Materials and Methods

Insect Collection and Rearing

S. frugiperda larvae were collected from Isabela, Philippines through the Institute of Plant Breeding, UPLB. The collected insect samples were reared in laboratory at room temperature conditions with photoperiod of 12 hours of light and dark photoperiod at 25oC room temperature. First generation FAW was used in the experiments. Following a 24-hour feeding period with insecticide-treated leaf discs, FAW larvae were subjected to total RNA extraction for expression analysis and gDNA extraction for amplification of CYP321A7 and CYP321A8. Four treatments were laid out for expression analysis, T1: those exposed to no insecticide treatment denoted as Control, T2: those exposed to Chlorantraniliprole denoted as CTPR, T3: those exposed to Thiamethoxam denoted as THMX, and T4: those exposed to an insecticide with dual active ingredients of Chlorantraniliprole and Thiamethoxam denoted as CTPR + THMX.

Chemicals

The insecticides used have an active ingredient of Chlorantraniliprole 5% SC, Thiamethoxam 25% WG, and dual active ingredient of Chlorantraniliprole 20% and Thiamethoxam 20% WG. Corn plants were sprayed with CTPR, THMX, and CTPR + THMX at 30 mL/16 L water, 4 g/16 L water, and 15 g/ 16 L water, respectively.

Primer Design

The selected Actin, CYP321A7 and CYP321A8 of Spodoptera frugiperda, as shown in Table 1, were obtained online from the National Center for Biotechnology Information (NCBI) website (https://www.ncbi.nlm.nih.gov/). The primer sequences were designed using primer-blast from NCBI (https://www.ncbi.nlm.nih.gov/tools/primer-blast/index.cgi?GROUP_TARGET=on) and dsRNA primers from SnapDragon (https://www.flyrnai.org/snapdragon) to obtain the forward and reverse sequences at 5’-3’. RNAi can be hindered by off-target effects, where the dsRNA molecule interacts with unintended genes with sequence similarity to the target. To mitigate this issue, platforms like SnapDragon implement a stringent base-pair identity threshold for the amplified region, minimizing the potential for off-target interactions (Kulkarni et al., 2006; Ma et al., 2006). Double stranded RNA for GFP was based on the available online sequence of mGFP (NCBI Accession no: L29345.1).

Relative Expression Analysis of CYP321A7 and CYP321A8 in Spodoptera frugiperda

Extraction of RNA and Preparation of cDNA

Total RNA was extracted from 3rd instar FAW larva exposed to CTPR, THMX and CTPR + THMX insecticides. FAW larvae Unexposed to insecticides were also isolated to act as control. The extraction was done using GF-1 Total RNA Extraction Kit (Vivantis, Shah Alam, Selangor Darul Ehsan, Malaysia) following the manufacturer’s protocol. Total RNA was extracted individually from ten insects per insecticide treatments and five insects for negative control. cDNA was subsequently synthesized from these RNA samples for the expression of CYP321A7 and CYP321A8 through sqRT-PCR using a thermal cycler (SimpliAmp, Applied Biosystem, Waltham, MA USA). First-strand cDNA synthesis was prepared from 1 μg of total RNA using the QuantiTect Reverse Transcription Kit (Qiagen, Hilden, Germany) following the manufacturer’s protocol. All synthesized cDNAs were stored at -20oC until use.

Expression of CYP321A7 & CYP321A8 Genes in CTPR, THMX and CTPR+THMX Exposed Larvae

The synthesized cDNAs were used as templates for two-step semi-quantitative RT-PCR with specific primers specific for CYP321A7 and CYP321A8 to determine their relative expression compared to Actin. The PCR mixture was prepared by putting up either CYP321A7 or CYP321A8 forward and reverse primers, GoTaq G2 (Promega, Fitchburg, WI, USA) colorless master mix. The cDNA template of 3 µL [150 ng] was used for the expression of CYP321A7, CYP321A8, and Actin. Actin was used as reference gene for this study as this gene was proved to show significant stability expression in FAW after insecticide treatment (Zhou et al., 2021). The PCR mixture, with a total of 10 µL volume, was run on a thermal cycler following synthesized primers’ protocol. The PCR products were subjected to electrophoresis at 50 V for 45 minutes, operating on an agarose gel with a concentration of 1.5%. The gels were stained with GelRed in 1X TAE buffer for 20 minutes and was destained for 10 minutes, followed by the digital capturing process through the BioBase gel documentation system (BIOBASE, Shandong, China). The Gel Pro Analyzer was utilized to conduct the quantitative analysis, while the band intensity was measured in relative absorbance units. The evaluation of expression of CYP450 in FAW was compared to the evaluation of the expression of Actin in the same insect sample. Mathematically speaking:
R e l a t i v e   C Y P 450   E x p r e s s i o n =   A b s o r b a n c e   a t   260   n m   C Y P 450   E x p r e s s i o n 1 − A b s o r b a n c e   a t   260   n m   A c t i n
Equation 1. Formula for correction of CYP450 expression. Modified from, “https://www.gene-quantification.de/strategy.html#slide.” Gene Quantification, 2004. Retrieved May 18, 2024.
This correction was done to normalize the possible variation in the sample concentration, as well as a control for reaction efficiency. It is important to note that some readings of Actin from the gel documentation system returned a value of 0, thereby resulting to errors. To rectify this situation, the reference formula from the literature cited was modified into Equation 1, such that the reference gene in the denominator was subtracted to 1. The corrected expression of Actin was also modified to be expressed in terms of percentage for easier interpretation and visualization of values.

Amplification and Sequence Alignment Analysis of CYP321A7 and CYP321A8 in Spodoptera frugiperda

Genomic DNA Extraction

The genomic DNA was extracted from 3rd instar FAW larvae exposed to CTPR, THMX and CTPR + THMX insecticides. Unexposed FAW larvae to insecticide were also isolated to act as control. The extraction was done using GF-1 Tissue DNA Extraction Kit (Vivantis, Shah Alam, Selangor Darul Ehsan, Malaysia) following the protocol recommended by the manufacturer for the extraction of the animal tissue. The procedure includes lysis, binding, washing and elution. For elution, 200 µl nuclease-free water was used and the gDNA was stored in -20oC until use. The concentrations of the gDNA, RNA, T7 PCR product template, and dsRNA samples were determined by UV spectrophotometry using BioDrop 125 cuvette (0.125mm pathlength) (Harvard Bioscience, Holliston, MA, USA) at 260/280 nm ratio absorbance.
Two gDNA isolates from each insecticide treatment and control were used for PCR. All PCR mixtures were then amplified using a thermal cycler (SimpliAmp, Applied Biosystem, Waltham, MA USA).

Amplification of CYP321A7 and CYP3218

The eluted gDNAs were used to amplify CYP321A7 and CYP321A8 using a two-step semi-quantitative RT-PCR. The PCR mixture was prepared by putting up either CYP321A7 or CYP321A8 forward and reverse primers, GoTaq G2 (Promega, Fitchburg, WI, USA) colorless master mix. The resulting mix was combined with 3 µL of eluted gDNA. The PCR mixture was amplified using a thermal cycler following synthesized primers’ protocol. The PCR products were subjected to electrophoresis at 50 V for 45 minutes, operating on an agarose gel with a concentration of 1.5%. The gels were stained with 1X GelRed (Biotium, CA, USA) in distilled water for 30 minutes and was destained for 10 minutes, followed by the digital capturing process through the BioBase gel documentation system (BIOBASE, Shandong, China).

Sequencing of the Purified PCR Products

The purified PCR products of CYP321A7 and CYP321A8 from gDNA of extracted FAW-CTPR exposed were upscaled to a final volume of 100 µL for sequencing analysis. The PCR mixture was prepared by putting up either CYP321A7 or CYP321A8 nuclease free-waster, forward and reverse primers, and GoTaq G2 colorless master mix. The resulting mix was combined with 3 µL gDNA template. The 3 µL of PCR products were checked on gel electrophoresis at 50 V for 45 minutes, operating on an agarose gel with a concentration of 1.5%. The same process was done for staining, destaining and image capturing of the gel as mentioned previously.
The remaining PCR products were run on gel electrophoresis following the same procedures as mentioned previously. The gel with amplicons has undergone purification using Gel and PCR Clean-up System Kit (Promega, Fitchburg, WI, USA). For elution, 50 µL of nuclease-free water was used. The purified PCR products were stored at -20oC until use.
The 25 µL purified PCR products were submitted to Macrogen (Seoul, Republic of Korea) and were analyzed for bi-directional sequencing using Capillary Electrophoresis (Sanger) Sequencing to verify the integrity of the sequence. The result sequences were then analyzed in BioEdit (version 7.7.1, Tom Hall) software to perform multiple sequence alignments and generate consensus sequences. The contigs were blast in NCBI to determine the query coverage, E-value, and percent identification. The contigs were submitted to NCBI through their submission portal (https://submit.ncbi.nlm.nih.gov/).

dsRNA Preparation

Synthesizing dsRNA

The primers for the target sequences, CYP321A7, CYP321A8, and GFP, were designed using and extended T7 polymerase promoter sequence at the 5’ ends of each strand. To amplify the target genes with extended T7 promoters, PCR mix was prepared by putting up together the forward and reverse primers, nuclease-free water, G2 GoTaq Colorless master mix to a final volume of 10 µL. The resulting mix was combined with 3 µL of purified PCR products of the amplified primers as template. The PCR mixture was amplified using a thermal cycler following synthesized primers’ protocol. The PCR product of CYP321A7 was diluted at 10x in nuclease-free water while CYP321A8 was used as is.
Amplification strategies of primers containing extended T7 promoter sequences included an initial 5 cycles at an annealing temperature of 5°C above the melting temperature of the gene-specific sequences, followed by 30 cycles of annealing approximately 5°C above the melting temperature of the entire primer, including the extended T7 promoter. The T7 PCR product templates were stored in -20°C until use. The T7 PCR product templates had also undergone sequencing analysis following the same procedures as mentioned previously.
For dsRNA preparation, purified PCR-generated templates from T7_CYP321A7, T7_CYP321A8, and T7_GFP were used DNA templates using T7 RiboMAX™ Express RNAi System Kit (Promega, Fitchburg, WI, USA). The RiboMAX Express T7 2x Buffer, DNA template, Enzyme Mix, T7 Express were mixed to obtain a final volume of 20 µL. Manufacturer’s protocol were then followed.
The concentration of T7 PCR product template and dsRNA samples were determined using UV spectrophotometry using BioDrop 125 cuvette (0.125mm pathlength) (Harvard Bioscience, Holliston, MA, USA) at 260/280 nm ratio absorbance. For dsRNA, it was diluted at 1:100 and was calculated using A260 absorbance to determine its concentration. The A260 value was divided by the pathlength used for the UV microvolume spectrophotometry then, multiplied with 1 unit of A260 nm multiplied to the dilution factor following multiplication to the total reaction after in vitro RNA transcription. Mathematically speaking;
d s R N A   c o n c e n t r a t i o n = A 260   v a l u e 0.0125 c m x   40   µ g m L x   d i l u t i o n   f a c t o r   x   t o t a l   I V T   r e a c t i o n
Equation 2. Calculation of dsRNA concentration using A260 nm absorbance.
The PCR products were subjected to electrophoresis at 100 V for 25 minutes, operating on an agarose gel with a concentration of 1.5%. The gels were stained with 1X GelRed (Biotium, CA, USA) in distilled water for 30 minutes and was destained for 10 minutes, followed by the digital capturing process through the BioBase gel documentation system (BIOBASE, Shandong, China).

Feeding Bioassay

Artificial Diet

The artificial diet solid mixture formulated was obtained at Institute of Plant Breeding, UPLB. The components of the solid mixture diet were ground corn, ground soybean, brewer’s yeast, wheat germ, ascorbic acid, vitamin E, multivitamins, methyl paraben, casein, choline chloride, sorbic acid and agar-agar.
The solid mixture was added to 350 mL of boiling distilled water and cooked for 10 minutes. While agar-agar was dissolved to 350 mL of boiling distilled water. Afterwards, it was mixed in a blender (Osterizer 4172, Oster, Philippines) to homogenize and grind further the solid components to bring a smooth texture of the diet.

LC50 of the Insecticide with Dual Active Ingredient of Chlorantraniliprole and Thiamethoxam

The lethal concentration of the selected insecticide was conducted prior to dsRNA feeding experiment to determine the concentration of the insecticide at 50% mortality. The insecticide used for this experiment was determined from the highest relative expression levels result. The 2nd instar FAW larvae (n=20) were exposed to the insecticide with concentrations of 36, 12, 4, 1.333, 0.444, 0.148, and 0.0493 ppm. The ppm was calculated using serial dilution sheet, a software developed by a private agrochemical company. The feeding bioassay experiment was done in 25oC room at 12-hour light and dark photoperiod.

Double-Stranded RNA (dsRNA) Feeding Bioassay

The larvae were given 1 µL [14 µg] of dsRNA solution. The artificial diet (0.7cm x 0.7cm x 0.7cm) was placed inside the hinged cups (23cm in height and 35cm in diameter) with holes in the cap. A moist tissue paper was also placed to keep the humidity inside the cup not so dry. A single drop of dsRNA solution of 1 µL was placed in the diet using a 2 µL pipette (Thermo Fisher Scientific, Waltham, MA, USA) for 24 hours followed by the exposure to an artificial diet supplemented with LC50 of CTPR + THMX insecticide after 48 hours. The artificial diet without insecticide was also used as a control. Each treatment consisted of a total 45 24-hr starved larvae, 3 replicates of 15 larvae each. The dsRNA-fed larvae mortality data were recorded at 24, 48, and 72 hours. Moribund status of larvae was used to assess the mortality rate. To evaluate the efficacy of RNAi-mediated knockdown of CYP321A7 and CYP321A8, 3 larvae from each triplicate per treatment were collected at 24 hours post exposure to insecticides.

Statistical Analysis

The lethal concentration from the mortality of bioassay data were estimated using Finney’s probit analysis spreadsheet calculator (Version 2021). The data for mortality was analyzed using IBM SPSS version 26. Test of significant difference was performed to compare percent mortality rate of larvae treated with different insecticides. To identify the most appropriate statistical test, assumptions such as normality and variance homogeneity were assessed. The Shapiro-Wilk test was employed to check the normality of the data, while Levene’s test was used to determine variance homogeneity. Since the data does not satisfy these assumptions, Kruskal-Wallis H-test and Dunn’s Test (post-hoc) was performed. Statistical tests were performed at a 5% level of significance.

Results

Relative Expression of CYP321A7 and CYP321A8 of FAW after Exposure to Insecticides

Expression patterns of CYP321A7 and CYP321A8 from FAW larvae exposed to CTPR, THMX and CTPR + THMX were analyzed by sqrRT-PCR. Figure 1 shows the relative expression levels of CYP321A7 and CYP321A8 in response to different insecticide treatments. In CTPR-exposed larvae, CYP321A7 shows a relatively high expression level with 2.69 compared to CYP321A8 with 1.46. However, both CYP450s had relatively low expression level compared to other THMX and CTPR+THMX. For larvae after exposure to THMX, CYP321A7 and CYP321A8 show an increased in expression as compared to CTPR – CYP321A7 had 4.90 while CYP321A8 had 6.03 expression levels. The CTPR+THMX insecticide treatments leads to the highest expression of both genes with 6.90 and 6.02, respectively. Furthermore, it revealed that CYP321A7 and CYP321A8 can only be overexpressed when induced with insecticides. In contrast to the relatively low expression of both CYP genes observed following CTPR exposure, the combined treatment of CTPR + THMX resulted in increased expression levels.
This observation indicates a potential synergistic effect of the two insecticides in detoxification mechanism of the CYP450 genes. This might suggest that the combination of these chemicals triggers a stronger response in FAW possibly as a mechanism to cope with increased toxicity. However, importantly, upregulation of CYP450 cannot be the sole reference to confer that the insect has gained resistant to a particular insecticide. The upregulation of CYP450s only indicates the insect’s enhanced metabolic potential to detoxify the insecticide (Yang et al., 2021).

Sequence Alignment Analysis of CYP321A7 and CYP321A8 in S. frugiperda

Following successful PCR amplification of CYP321A7 and CYP321A8, the PCR products were purified and were subjected to Sanger sequencing for subsequent sequence analysis. As shown in Table 2, the analysis revealed 100% query coverage, an E-value of 0, and 100% identity between the FAW CYP321A7 gene (PP693211.1) and the reference sequence (MZ945565.1) from Chen et al. (2022). Homologous genes from S. litura (MF802804.1; Wang et al., 2017), S. littoralis (LR82540.2; King, 2020), and S. exigua (KX443442.1; Hu et al., 2019) showed progressively lower percent identities (87.88%, 86.37%, 83.49%, respectively) compared to S. frugiperda, indicating increasing evolutionary divergence. The Agrochola lychnidis (OY798656.1; WSTLP, 2023) exhibited the lowest similarity (query cover 89% and identity 77.69%).
On the other hand, Table 3 shows the comparison of the CYP321A8 gene from Spodoptera frugiperda (accession number PP693211.1) with its homologs identified in other organisms. The S. frugiperda (accession number MZ945600.1; Chen et al., 2022) serves as the reference exhibited a complete query cover, E-value of 0, and 100% identity. Homologous genes from S. littoralis (LR82540.2; King, 2020), S. litura (XM_022969704.1; Anonymous), and S. exigua (LR824610.2; King, 2020) showed progressively lower percent identities (90.60%, 89.66%, 86.98%, respectively) compared to S. frugiperda, indicating increasing evolutionary divergence. The Agrochola lychnidis (OY798656.1; WSTLP, 2023) exhibited the lowest similarity (query cover 95% and identity 77.79%).
Overall, sequence analysis revealed 100% identity between the obtained CYP321A7 and CYP321A8 sequences and their corresponding reference sequences deposited in NCBI with accession numbers MZ945565.1 and MZ945600.1, respectively. This suggests that the target CYP450s recovered from gDNA of S. frugiperda collected from the Philippines used in this study were 100% identical or similar to the reference sequence published in GenBank database.

The Integrity of Resulting dsRNAs

The integrity of dsCYP321A7, dsCYP321A8 and dsGFP were analyzed in 1.5% agarose gel electrophoresis ran at 100 V for 25 mins which showed the expected size bands of 268, 274, 352 bp, respectively.

RNAi-Mediated Downregulation of dsCYP321A7 and dsCYP321A8 from S. frugiperda via sqRT-PCR

The results, as shown in Table 4, revealed that knockdown of CYP321A7 and CYP321A8 increased the sensitivity to the insecticide with higher mortalities compared with control (P < 0.05; n = 5) and C + T (CTPR + THMX) insecticide treatment only. It was significantly higher in dsCYP321A7-fed 2nd instar larvae compared dsGFP (control) after RNAi at 24 hours, then exposed to CTPR + THMX. While there is no significant difference in mortality rate of dsCYP321A8-fed 2nd instar larvae compared with dsGFP after RNAi at 24 hours, then exposed to CTPR + THMX. Collectively, the results showed that FAW larvae exposed to Chlorantraniliprole + Thiamethoxam insecticide increases its susceptibility after dsRNA feeding of dsCYP321A7 and dsCYP321A8.
The expression of CYP321A8 on insect samples treated with dsCYP321A8 and dsGFP were analyzed using sqRT-PCR. Figure 2 shows that there is a decrease in the expression level of CYP321A8 for samples treated with dsCYP321A8 compared to the control, dsGFP after 24 hours post exposure to insecticide.
Figure 3 shows the phenotypic effects to dsRNA-fed larvae after exposure to insecticide at 48 hours. dsRNA-fed larvae after exposure to insecticide had not develop. As observed 2 days post exposure to insecticide, the larvae were not feeding the artificial diet supplemented. In a study of the effects of Chlorantraniliprole to nutritional indices, the relative growth rate and digestibility significantly decreases after exposure of the insect to Chlorantraniliprole (He et al., 2019). Additionally, seed treatments containing thiamethoxam and chlorantraniliprole as active ingredients reduced fall armyworm leaf consumption in soybeans (Gontijo et al., 2018). It also extends the larval duration resulted in reduced average weights for both larvae and pupae, along with decreased rates of pupation and emergence (He et al., 2019).
The larvae fed with dsCYP321A7 and dsCYP321A8 show an evident response to dsRNA treatments, depending on the feeding period. It is noteworthy that dsRNA fed larvae continued its growth while the dsRNA-fed larvae post insecticide treatment did not develop due to increased susceptibility of the insecticide after feeding of artificial diet supplemented with dsRNAs. The dsGFP-fed larvae, a control treatment, and larvae showed much less effect from the insecticide.
These observations suggest that RNAi targeting CYP321A7 and CYP321A8 genes has the potential to increase susceptibility of FAW larvae to insecticides. This could lead to reduced larval viability and mitigate the development of insecticide resistance. This research highlights the potential of integrating RNAi technology into novel pest control strategies that target insect detoxification mechanisms.

DISCUSSION

Fall armyworm (FAW) is a destructive pest that has rapidly spread since its first invasion in 2016. While various control methods exist, farmers often rely on insecticides, leading to concerns about resistance. RNA interference (RNAi) offers a promising alternative. This technique effectively regulates gene expression and has shown potential in pest control, making it a valuable tool for developing new FAW management strategies. In this study, CYP321A7 and CYP321A8 of FAW were evaluated to determine the efficiency of RNAi in knocking down CYP450 genes after exposure to insecticide with dual active ingredient of Chlorantraniliprole and Thiamethoxam. These CYP450 genes were found to be expressed after exposure to insecticides (Bai-Zhong et al. 2020; Hafeez et al., 2022)
Cytochrome P450 (CYP450) genes can be found in nearly all living things, including bacteria, protists, plants, fungi, and animals (Feyereisen, 2012). The increased synthesis of metabolic enzymes that detoxify or sequester pesticides before they reach the target site is one of the molecular changes that are usually associated with resistant insect populations (Feyereisen, 2012; Yang, et al., 2020). Enhanced metabolic detoxification of xenobiotics in insects correlates closely with the upregulation of CYP450 protein production and enzymatic activities. Both the induction and constitutive overexpression of insect CYP450s play key roles in detoxifying xenobiotics and facilitating adaptation to fluctuating environments (Lu et al., 2021). Numerous key CYP450 genes in Lepidoptera have been associated with various insecticide resistance mechanisms. These include CYP321A7 and CYP321A8 in Spodoptera frugiperda (Bai-Zhong, et al., 2020; Hafeez, et al., 2022).
FAW populations can resist insecticides through several mechanisms. One of them being rapid detoxification by cytochrome P450 monooxygenases (CYP450s) (Lu et al., 2021). Overexpression of some of these CYP450s by the insect leads to an accelerated rate of metabolism, which results in inactivation and, hence, a reduction in the efficacy of the insecticides (Hafeez et al., 2022; Lu et al., 2021). Additionally, insecticide use can create a potent selective pressure, driving the evolution of resistance in fall armyworm populations. This resistance can arise through various mechanisms at the genetic and protein level. At genetic level, new genes may evolve, or mutations can occur in the promoter regions of existing genes. These promoter mutations can alter gene expression, potentially leading to higher expression levels of enzymes that detoxify insecticides. Alternatively, mutations within protein-coding regions can alter the amino acid sequence of the encoded protein. These changes in protein structure can directly impact the ability of the protein to bind insecticides or perform its normal function, rendering the insecticide ineffective. Finally, even without changes in the protein sequence, modifications like phosphorylation can influence enzyme activity, further contributing to resistance development (Ye et al., 2022).
Sustainable pest management is continually challenged with insect resistance to synthetic insecticides (Hafeez, et al., 2022). Developing pesticide resistance management techniques requires a thorough understanding of the mechanisms through which insects acquire resistance to insecticides (Siddiqui et al., 2023). Repeated use of chemicals would increase the risk of insect resistance to chemicals. Thus, the demand to innovate approaches in controlling pests is highly encouraged. Using RNA interference (RNAi) would open new opportunities for FAW management. The concept of RNAi gained prominence after Fire and colleagues’ seminal discovery, which definitively elucidated the biochemical mechanism of gene silencing by introducing purified double-stranded RNA (dsRNA) directly into Caenorhabditis elegans (Fire et al., 1998). RNAi uses dsRNA molecules as triggers to direct homology-dependent, post-transcriptional mechanism of gene silencing. The primary mechanism utilized for the study and management of insects is the short interfering RNA (siRNA) pathway, whose biological function is to resist against exogenous dsRNA (Niebres & Alviar, 2023).
Various methods for applying exogenous dsRNAs, siRNAs, and hpRNAs to plants for targeted gene silencing include spraying, infiltration, injection, spreading, mechanical inoculation, and soaking of roots or seeds. These techniques are broadly utilized to deliver RNA molecules onto plants effectively (Das & Sherif, 2020). GreenLight Biosciences’ Calantha (Ledprona) is the first sprayable biopesticide product based on double-stranded RNA targets the Proteasome Subunit Beta Type-5 in the Colorado Potato Beetle (Leptinotarsa decemlineata). It works by "silencing" a crucial gene necessary for the beetle’s survival, effectively controlling this pest without producing a genetically modified organism (Rodrigues et al., 2021). As of December 2023, the biopesticide has granted registration under the Federal Insecticide, Fungicide, and Rodenticide Act of USA (ID: EPA-HQ-OPP-2021-0271-0194). Ledprona can now also be retrieved in Insecticide Resistance Action Committee with group no. of 35, grouped as protein suppressor with mode of action of microbial disruptors of insect midgut membrane (IRAC, 2024). The Bayer “SmartStax Pro” maize (Mon87411), a plant-incorporated protectant, which combines the expression of the Bacillus thuringiensis (Bt) Cry3Bt1 toxin with glyphosphate resistance and the expression of a dsRNA that targets the Snf7 gene of the western corn rootworm (Diabrotica virgifera virgifera). RNA interference-mediated silencing of this gene involved in the transport of transmembrane proteins causes mortality of D. v. virgifera which leads to reducing root damage in corn (De Schutter, et al., 2022).
Numerous studies already shown the efficacy of RNAi technology in controlling insect pest as well as diseases in laboratory set ups. To list, study of Hafeez, at al. (2022) revealed that droplet feeding of dsRNAs (CYP321A7 and CYP6AE43) via artificial diet significantly increased mortality rates of indoxacarb-resistant FAW larvae. Also, Bai-Zhong, et al. (2020) successfully demonstrated RNAi by feeding dsRNA (CYP321A8, CYP321B1, and CYP321A9) and results showed that the second-instar larvae became more sensitive to chlorantraniliprole. Zhang, et al. (2010) proved that chitosan/double-stranded RNA nanoparticles might, therefore, be an effective mediator in RNA interference (RNAi) in mosquito larvae to the chitin synthase genes (AgCHS1 and AgCHS2) by feeding the larvae with these nanoparticles resulted in downregulated transcript abundance by significant folds of AgCHS1.
Successful applications of RNAi to silence genes critical for pest survival and reproduction, such as those involved in growth, development, and fecundity had been studied. The results are promising for the development of RNAi as a tool for pest control, with various delivery methods such as microinjection, oral ingestion, and transgenic plants being tested. Systemic RNAi, where the effect of RNAi spreads throughout the organism, has been shown to be effective in coleopteran species, although it varies among other insect groups. Challenges in applying RNAi technology, including variable RNAi efficiency across different insect species, the concern that insects may evolve resistance to dsRNA-based products, and the need for efficient delivery systems that protect dsRNA from degradation. Overall, the findings suggest that while RNAi holds significant potential for targeted pest management and gene functional analysis, several technological and biological hurdles need to be addressed to enhance its efficacy and application scope (Zhu & Palli, 2020).

CONCLUSION

The sensitivity of S. frugiperda to the insecticide with dual active ingredient of Chlorantraniliprole and Thiamethoxam was increased after introduction of dsCYP321A7 [14.72 µg/µL] and dsCYP321A8 [14.08 µg/µL] to the 2nd instar FAW larva by feeding with artificial diet.

Acknowledgments

This research was supported by Department of Science and Technology - Accelerated Science and Technology Human Resource Development Program – Student Research Support Fund. We acknowledge the members of D110 Insect Vector-Pathogen-Plant Interaction Laboratory cohort 2023-2024, at the University of the Philippines Los Baños (UPLB) for the unwavering support which has been instrumental in this experiment.

References

  1. [USAID] United States Agency for International Development. 2018. Feed the Future. Retrieved from Fall armyworm (FAW) management report: evaluating least toxic and cost-effective approaches to FAW management: https://pdf.usaid.gov/pdf_docs/PA00WF1P.pdf.
  2. [IRAC] INSECTICIDE RESISTANCE ACTION COMMITTEE. 2024. Mode of action classification scheme. Retrieved on April 24, 2024, from https://irac-online.org/documents/moa-classification/.
  3. AGRAWAL N., DASARADHI PVN, MOHMMED A, MALHOTRA P, BHATNAGAR RK, MUKHERJEE SK. 2003. RNA interference: Biology, mechanism, and applications. Microbiology and Molecular Biology Reviews, 67(4), 657–685. [CrossRef]
  4. BAI-ZHONG Z, XU S, CONG-AI Z, LIU-YANG L, YA-SHE L, XING G, DONG-MEI C, ZHANG P, MING-WANG M, & XI-LING C. 2020. Silencing of cytochrome P450 in Spodoptera frugiperda (Lepidoptera: Noctuidae) by RNA interference enhances susceptibility to chlorantraniliprole. Journal of Insect Science, 20(3). [CrossRef]
  5. BERGE J-B, RENE F, AMICHOT M. 1998. Cytochrome P450 monooxygenases and insecticide resistance in insects. Philosophical Transactions of the Royal Society of London B: Biological Sciences, 353(1376), 1701-1705. [CrossRef]
  6. CAPINERA J. 2020. Fall armyworm. Retrieved from Featured Creatures on April 20, 2024, at https://entnemdept.ufl.edu/creatures/field/fall_armyworm.htm.
  7. CHEN H, XIE M, LIN L, ZHONG Y, ZHANG F, SU W. 2022. Transcriptome analysis of detoxification-related genes in Spodoptera frugiperda (Lepidoptera: Noctuidae). Journal of Insect Science, 22(1). [CrossRef]
  8. DAS PR, SHERIF SM. 2020. Application of exogenous dsRNAs-induced RNAi in agriculture: Challenges and triumphs. In Frontiers in Plant Science (Vol. 11). Frontiers Media S.A. [CrossRef]
  9. DAY R, ABRAHAMS P, BATEMAN M, BEALE T, CLOTTEY V, COCK M. 2017. Fall armyworm: Impacts and implications for Africa. Outlooks on Pest Management, 28(5). [CrossRef]
  10. DE SCHUTTER K, TANING CNT, VAN DAELE L, VAN DAMME EJM, DUBRUEL P, SMAGGHE G. 2022. RNAi-based biocontrol products: Market status, regulatory aspects, and risk assessment. Frontiers in Insect Science, 1. [CrossRef]
  11. FEYEREISEN R. 2012. Insect CYP genes and P450 enzymes. In Insect Molecular Biology and Biochemistry (pp. 236-316). Academic Press. [CrossRef]
  12. FIRE A, XU S, MONTGOMERY MK, KOSTAS SA, DRIVER SE, MELLO CC. 1998. Potent and specific genetic interference by double-stranded RNA in Caenorhabditis elegans. Nature, 391(6669), 806–811. [CrossRef]
  13. GUENGERICH FP. 2018. Mechanisms of cytochrome P450-catalyzed oxidations. ACS Catalysis, 8(12), 10964–10976. [CrossRef]
  14. HAFEEZ M, LI X, ULLAH F, ZHANG Z, ZHANG J, HUANG J, FERNÁNDEZ-GRANDON GM, KHAN MM, SIDDIQUI JA, CHEN L, REN XY, ZHOU S, LOU Y, LU Y. 2022. Down-regulation of P450 genes enhances susceptibility to indoxacarb and alters physiology and development of fall armyworm, Spodoptera frugiperda (Lepidoptera: Noctuidae). Frontiers in Physiology, 13. [CrossRef]
  15. HASNAIN A, ZHANG S, CHEN Q, XIA L, WU Y, GONG C, et al. 2023. Effects of chlorantraniliprole on the life history traits of fall armyworm Spodoptera frugiperda (Lepidoptera: Noctuidae). Frontiers in Physiology. [CrossRef]
  16. HU B, ZHANG SH, REN MM, TIAN XR, WEI Q, MBURU DK, SU JY. 2019. The expression of Spodoptera exigua P450 and UGT genes: Tissue specificity and response to insecticides. Insect Science, 26(2), 199–216. [CrossRef]
  17. JOGA M, ZOTTI M, SMAGGHE G, CHRISTIAENS O. 2016. RNAi efficiency, systemic properties, and novel delivery methods for pest insect control: What we know so far. Frontiers in Physiology, 7, 553. [CrossRef]
  18. KUMAR RM, GADRATAGI BG, PARAMESH V, KUMAR P, MADIVALAR Y, NARAYANAPPA N, ULLAH F. 2022. Sustainable management of invasive fall armyworm, Spodoptera frugiperda. Agronomy, 12(9). [CrossRef]
  19. LI Y, WANG Z, ROMEIS J. 2021. Managing the invasive fall armyworm through biotech crops: A Chinese perspective. Trends in Biotechnology, 39(2), 105-107. [CrossRef]
  20. LU K, SONG Y, ZENG R. 2021. The role of cytochrome P450-mediated detoxification in insect adaptation to xenobiotics. Current Opinion in Insect Science, 43, 103–107. [CrossRef]
  21. MATOVA PM, KAMUTANDO CN, MAGOROKOSHO C, KUTYWAYO D, GUTSA F, LABUSCHAGNE M. 2020. Fall armyworm invasion, control practices, and resistance breeding in Sub-Saharan Africa. Crop Science, 60(6), 2951–2970. [CrossRef]
  22. NAVASERO M, MARCELA N, ARIES G, BURGONIO G, ARDEZ, K, EBUENGA M, et al. 2020. Detection of the fall armyworm, Spodoptera frugiperda (J.E. Smith) (Lepidoptera: Noctuidae) using larval morphological characters, and observations on its current local distribution in the Philippines. The Philippine Entomologist, 33(2), 171-184.
  23. NIEBRES C, ALVIAR KB. 2023. Disruption of transmission of plant pathogens in the insect order Hemiptera using recent advances in RNA interference biotechnology. Archives of Insect Biochemistry and Physiology, 113(4). [CrossRef]
  24. NITNAVARE RB, BHATTACHARYA J, SINGH S, KOUR A, HAWKESFORD MJ, ARORA N. 2021. Next generation dsRNA-based insect control: Success so far and challenges. Frontiers in Plant Science, 12. [CrossRef]
  25. NWANZE JAC, BOB-MANUEL RB, ZAKKA U, KINGSLEY-UMANA EB. 2021. Population dynamics of fall armyworm (Spodoptera frugiperda J.E. Smith) (Lepidoptera: Noctuidae) in maize-cassava intercrop using pheromone traps in Niger Delta Region. Bulletin of the National Research Centre, 45(1). [CrossRef]
  26. OMWOYO CO, MBURU J, NZUVE F, NDERITU J. 2022. Assessment of maize yield losses due to the effect of fall armyworm (Spodoptera frugiperda) infestation: The case of Trans-Nzoia County, Kenya. International Journal of Pest Management. [CrossRef]
  27. PHAMBALA K, TEMBO Y, KASAMBALA T, KABAMBE VH, STEVENSON PC, BELMAIN SR. 2020. Bioactivity of common pesticidal plants on fall armyworm larvae (Spodoptera frugiperda). Plants (Basel, Switzerland), 9(1). [CrossRef]
  28. RODRIGUES TB, MISHRA SK, SRIDHARAN K, BARNES ER, ALYOKHIN A, TUTTLE R, KOKULAPALAN W, GARBY D, SKIZIM NJ, TANG YW, MANLEY B, AULISA L, FLANNAGAN RD, COBB C, NARVA KE. 2021. First sprayable double-stranded RNA-based biopesticide product targets proteasome subunit beta type-5 in Colorado potato beetle (Leptinotarsa decemlineata). Frontiers in Plant Science, 12. [CrossRef]
  29. SABERI E, MONDAL M, PAREDES-MONTERO JR, NAWAZ K, BROWN JK, QURESHI JA. 2024. Optimal dsRNA concentration for RNA interference in Asian citrus psyllid. Insects, 15(1), 58. [CrossRef]
  30. SCOTT JG. 1999. Cytochromes P450 and insecticide resistance. In Insect Biochemistry and Molecular Biology (Vol. 29). https://www.elsevier.com/locate/ibmb. [CrossRef]
  31. SIDDIQUI JA, FAN R, NAZ H, BAMISILE BS, HAFEEZ M, GHANI MI, WEI Y, XU Y, CHEN X. 2023. Insights into insecticide-resistance mechanisms in invasive species: Challenges and control strategies. Frontiers in Physiology, 13. [CrossRef]
  32. WANG RL, HE YN, STAEHELIN C, LIU SW, SU YJ, ZHANG JE. 2017. Identification of two cytochrome monooxygenase P450 genes, CYP321A7 and CYP321A9, from the tobacco cutworm moth (Spodoptera litura) and their expression in response to plant allelochemicals. International Journal of Molecular Sciences, 18(11). [CrossRef]
  33. YANG X, DENG S, WEI X, YANG J, ZHAO Q, YIN C, et al. 2020. MAPK-directed activation of the whitefly transcription factor CREB leads to P450-mediated imidacloprid resistance. Proceedings of the National Academy of Sciences of the United States of America, 117(19), 10246–10253. [CrossRef]
  34. YANG XM, SONG YF, SUN XX, SHEN XJ, WU QL, ZHANG HW, et al. 2021. Population occurrence of the fall armyworm, Spodoptera frugiperda (Lepidoptera: Noctuidae), in the winter season of China. Journal of Integrative Agriculture, 20(3), 772-782. [CrossRef]
  35. YAO Y, LIN DJ, CAI XY, WANG R, HOU YM, HU CH, et al. 2022. Multiple dsRNases involved in exogenous dsRNA degradation of fall armyworm Spodoptera frugiperda. Frontiers in Physiology. [CrossRef]
  36. YE M, NAYAK B, XIONG L, XIE C, DONG Y, YOU M, et al. 2022. The role of insect cytochrome P450s in mediating insecticide resistance. Agriculture (Switzerland), 12(1). [CrossRef]
  37. ZHANG X, ZHANG J, ZHU KY. 2010. Chitosan/double-stranded RNA nanoparticle-mediated RNA interference to silence chitin synthase genes through larval feeding in the African malaria mosquito (Anopheles gambiae). Insect Molecular Biology, 19(5), 683–693. [CrossRef]
  38. ZHANG Y, XU L, LI S, ZHANG J. 2019. Bacteria-mediated RNA interference for management of Plagiodera versicolora (Coleoptera: Chrysomelidae). Insects, 10(12). [CrossRef]
  39. ZHOU L, MENG JY, RUAN HY, YANG CL, ZHANG CY. 2021. Expression stability of candidate RT-qPCR housekeeping genes in Spodoptera frugiperda (Lepidoptera: Noctuidae). Archives of Insect Biochemistry and Physiology, 108(1). [CrossRef]
  40. ZHU KY, PALLI SR. 2020. Mechanisms, applications, and challenges of insect RNA interference. Annual Review of Entomology, 65, 293–311. [CrossRef]
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Figure 1. Relative Expression levels of CYP321A7 and CYP321A8 to actin after exposure to various insecticides.
Figure 1. Relative Expression levels of CYP321A7 and CYP321A8 to actin after exposure to various insecticides.
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Figure 2. Expression CYP321A8 after of dsGFP and dsCYP321A8 RNAi-mediated knockdown in FAW.
Figure 2. Expression CYP321A8 after of dsGFP and dsCYP321A8 RNAi-mediated knockdown in FAW.
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Figure 3. dsRNA-fed larvae after exposure to insecticide at 48 hours. (A) dsCYP321A7-fed FAW larvae after 72 hours. (B) dsCYP321A7-fed FAW larvae after exposure to insecticide at 48 hours. (C) dsCYP321A8-fed FAW larvae after 72 hours. (D) dsCYP321A8-fed FAW larvae after exposure to insecticide at 48 hours. (E) dsGFP-fed FAW larvae after exposure to insecticide at 48 hours. (F) dsGFP-fed FAW larvae after exposure to insecticide at 48 hours. (G) Unexposed FAW larvae.
Figure 3. dsRNA-fed larvae after exposure to insecticide at 48 hours. (A) dsCYP321A7-fed FAW larvae after 72 hours. (B) dsCYP321A7-fed FAW larvae after exposure to insecticide at 48 hours. (C) dsCYP321A8-fed FAW larvae after 72 hours. (D) dsCYP321A8-fed FAW larvae after exposure to insecticide at 48 hours. (E) dsGFP-fed FAW larvae after exposure to insecticide at 48 hours. (F) dsGFP-fed FAW larvae after exposure to insecticide at 48 hours. (G) Unexposed FAW larvae.
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Table 1. Primer design using NCBI Primer-blast and SnapDragon dsRNA synthesis tools.
Table 1. Primer design using NCBI Primer-blast and SnapDragon dsRNA synthesis tools.
NAME ACCES-SION NO. PURPOSE PRIMER SEQUENCE
5’-3’		 TM (OC) FRAGMENT LENGTH (bp)
CYP
321A7 		MZ945565.1 sqRT-PCR F:GGGACCAATGTGGGACTTCA 64.0 807
R: GCATTAGCACAAGGCTCCAC 60.5
dsRNA synthesis F: AAGATGGAAGCTGATGCGAT 57.8 268
T7F: GGATCCTAATACGACTCACTATAGGAAGATGGAAGCTGATGCGAT 68.9
R: ATTGAGTTCGTTCCAATGCC 57.7
T7R: GGATCCTAATACGACTCACTATAGGATTGAGTTCGTTCCAATGCC 68.8
RNAi knockdown F: TGGTGCACGTCTTACGAAAC 59.5 262
R: GGGAAAATGCCACCTCTGTA 60.2
CYP
321A8 		MZ945600.1 sqRT-PCR F: GCTACTGGAAAAAGCGTGGC 60.9 849
R: CACAAGGCTCTACACCAGCA 61.8
dsRNA synthesis F: ATTTCATAACACAGCGTGCG 59.9 274
T7F: GGATCCTAATACGACTCACTATAGGATTTCATAACACAGCGTGCG 68.0
R: GCCGTAAACAACGGAGTCAT 59.0
T7R: GGATCCTAATACGACTCACTATAGGGCCGTAAACAACGGAGTCAT 70.4
RNAi knockdown F: AAGGTGCTGAGTGAAGCGAT 60.4 258
R: TATACACGTCCTGTTGCCCA 60.5
Actin OK319028.1 sqRT-PCR F: AGCTGAGGGCTATGTAATTG 55.4 490
R: AACAGTCCTCTTGATGTCAC 56.6
mGFP dsRNA synthesis F: ATGGTAGATCTGACTAGTAAAG 48.6 352
T7F: GAATTCTAATACGACTCACTATAGGGAGATGAGGGATACGTGCAGGAGA
R: TCACACGTGGTGGTGGTGGTG 62.2
T7R: GAATTCTAATACGACTCACTATAGGGAGATGCCGTTCTTTTGCTTGTCG
Table 2. Homology of Spodoptera frugiperda’s CYP321A7.
Table 2. Homology of Spodoptera frugiperda’s CYP321A7.
GENE ORGANISM ACCESSION NO. QUERY COVER E VALUE PERCENT IDENTITY
CYP321A7

PP693210.1
(dela Cruz, R.K.D. & Alviar, K.B., 2024)		 Spodoptera frugiperda MZ945565.1
(Chen et al., 2022)		 100% 0 100%
Spodoptera litura MF802804.1
(R. L. Wang et al., 2017)		 97% 0 87.88%
Spodoptera littoralis LR824540.2
(King, 2020)		 100% 0 86.37%
Spodoptera exigua KX443442.1
(Hu et al., 2019)		 100% 0 83.49%
Agrochola lychnidis OY796856.1
(WSTLP, 2023)*		 89% 0 77.69%
*Wellcome Sanger Tree of Life Programme.
Table 3. Homology of Spodoptera frugiperda’s CYP321A8.
Table 3. Homology of Spodoptera frugiperda’s CYP321A8.
GENE ORGANISM ACCESSION NO. QUERY COVER E VALUE % IDENTITY
CYP321A8

PP693211.1
(dela Cruz, R.K.D. & Alviar, K.B., 2024)		 Spodoptera frugiperda MZ945600.1
(Chen et al., 2022)		 100% 0 100%
Spodoptera littoralis LR824540.2
(King, 2020)		 100% 0 90.60%
Spodoptera litura XM_022969704.1
(Anonymous)		 98% 0 89.66%
Spodoptera exigua LR824610.2
(King, 2020)		 100% 0 86.98%
Agrochola lychnidis OY796856.1
(WSTLP, 2023)*		 95% 0 77.79%
*Wellcome Sanger Tree of Life Programme.
Table 4. Mortality Rate of dsRNA-fed S. frugiperda larvae after exposure to CTPR+THMX.
Table 4. Mortality Rate of dsRNA-fed S. frugiperda larvae after exposure to CTPR+THMX.
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