Next Article in Journal
Optimization of Mapping Tools and Investigation of Ribosomal RNA Influence for Data-Driven Gene Expression Analysis in Complex Microbiomes
Previous Article in Journal
Bacillus multifaciens sp. nov., a Crucial and Highly-Active Flavor and Protease Producer Isolated from the qu-Starter of Chinese Wuliangye Baijiu
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Microorganisms
Volume 13
Issue 5
10.3390/microorganisms13050994
microorganisms-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

The Developmental Disorders of Fall Armyworm (Spodoptera frugiperda, Lepidoptera: Noctuidae) Caused by the Infection with Nosema sp. (Microsporidia: Nosematidae)

by
Yudi Xu
,
Haoyu Liu
,
Xinzheng Huang
,
Shuqian Tan
* and
Wangpeng Shi
*
MOA Key Lab of Pest Monitoring and Green Management, Department of Entomology, China Agricultural University, Beijing 100193, China
*
Authors to whom correspondence should be addressed.
Microorganisms 2025, 13(5), 994; https://doi.org/10.3390/microorganisms13050994
Submission received: 7 March 2025 / Revised: 21 April 2025 / Accepted: 24 April 2025 / Published: 26 April 2025
(This article belongs to the Section Molecular Microbiology and Immunology)
Browse Figures
Versions Notes

Abstract

:
The fall armyworm (Spodoptera frugiperda), a globally invasive pest, poses substantial threats to corn in China. Microsporidia are a group of obligate intracellular parasitic fungi and are considered to have great potential in biological control. In this article, we investigated the pathology of Nosema sp. infection in S. frugiperda larvae at the organismal, cellular, and molecular levels. At the organism level, this microsporidian significantly prolonged the developmental duration of the host, reduced its body weight, caused molting failure, and led to a high mortality rate at 98.9%, 97.8%, and 64.0%, respectively, in 5 × 105, 5 × 104, 5 × 103 spores/larva doses. Microsporidia infection caused severe damage to midgut cells, including the formation of vacuoles in the cytoplasm, mitochondria, and intercellular spaces, destruction of goblet cells, and partial encapsulation of spores by mitochondria. Transcriptomic profiling revealed significant alterations in gene expression profiles in S. frugiperda larvae following microsporidian infection. The expression levels of genes associated with the chitin synthesis pathway (CHS1, G6PI, GFAT, GNPNA, PAGM, UAP) were inhibited, which may contribute to the effects of Nosema sp. on the growth and development of S. frugiperda.

1. Introduction

The fall armyworm (Spodoptera frugiperda), a globally distributed agricultural pest originating from the Americas, has posed severe threats to China’s food security since its invasion in 2019 [1]. Characterized by strong migratory capacity, high fecundity, broad host range, and voracious feeding habits, this pest has caused significant damage to China’s corn production and has been classified as a Class I crop pest in China [2,3]. While chemical control remains effective in managing fall armyworm infestations, it carries the risk of inducing pesticide resistance [4]. In contrast, biological control offers distinct advantages including environmentally friendly, long-term effectiveness, and low resistance risk. Recent advances in biological control strategies against fall armyworms have been achieved through the application of various natural enemies and pathogens, including parasitic wasps, Beauveria bassiana, Metarhizium anisopliae, Bacillus thuringiensis, nucleopolyhedroviruses (NPVs), and microsporidia [5,6,7,8].
Microsporidia are obligate intracellular parasitic fungi ubiquitously distributed across nearly all vertebrates and invertebrates, particularly insects [9]. Entomopathogenic microsporidian species are considered promising agents for biological control [10]. Microsporidia infections in insects could cause multi-level pathological effects. At the organismal level, infected individuals exhibit altered color, developmental stunting, morphological aberrations, and behavioral modifications compared to healthy counterparts [8,10,11,12]. At the cellular level, infection induces cytopathological effects, including cell and nuclear hypertrophy, vacuolation, xenomas, and apoptosis dysregulation [10,13,14]. At the molecular level, microsporidian parasitism triggers extensive transcriptomic reprogramming, significantly altering host gene expression profiles [15]; for example, infection of Bombyx mori by Nosema bombycis alters expression of genes governing juvenile hormone (JH) biosynthesis and immune pathways, critical regulators of silkworm development [16]. The genes that regulate the cell cycle are modulated when bees are infected by microsporidia [17]. Tribolium castaneum infected by Paranosema whitei, the chitin metabolic genes changed [18].
As a fundamental structural biopolymer, chitin serves critical roles in insect exoskeletons, tracheal systems, internal tendon structures, and intestinal peritrophic matrices [19]. Its biosynthesis pathway involves eight key enzymatic steps mediated sequentially by: trehalase (TRE), hexokinase (HK), glucose-6-phosphate isomerase (G6PI), glutamine-fructose-6-phosphate aminotransferase (GFAT), glucosamine-6-phosphate N-acetyltransferase (GNPNA), phosphoacetylglucosamine mutase (PAGM), UDP-N-acetylglucosamine pyrophosphorylase (UAP), and chitin synthase (CHS) [20]. There are two types of chitin synthases in most insects. Among them, CHS1 is mainly present in the cuticle and trachea, while CHS2 is present in the peritrophic membrane. CHS plays an important role in growth and development, molting, and pupation [19]. CHS1 is regulated by various factors, including hormones (e.g., 20E), cuticle damage, carbohydrate metabolism, miRNAs, and chitin synthesis inhibitors [21,22,23]. The infection of the host by microsporidia can have an impact on chitin metabolism [18], but there is currently no report on its effect on chitin synthesis.
In this article, we evaluated developmental impacts on fall armyworm larvae infected by Nosema sp., and ultrastructural histopathological analysis was exhibited. At the molecular level, transcriptomic profiling coupled with targeted validation identified significant regulatory alterations in chitin synthesis pathways.

2. Materials and Methods

2.1. Insects and Microsporidia

The fall armyworm larvae were bought from Henan Jiyuan Baiyun Industry Co., Ltd. (Jiyuan, China) and kept in insect rearing room (27 ± 2 °C, 60 ± 5% humidity and 14:10 photoperiod) for at least 5 generations. For spore production, 4th instar larvae were starved for 6–8 h and fed with artificial diets (2 mm × 2 mm × 2 mm) polluted by Microsporidia. After the diets were consumed, the larvae were fed with clean diets. The dead larvae were collected and homogenized in sterilized distilled water, and the homogenate was filtered through absorbent gauze. The spore filtrate was purified by 90% Percoll gradient centrifugation, the spore pellet was resuspended in sterilized distilled water and stored at 4 °C until further use [24].

2.2. Latent Period Detect

Three concentrations (1 × 109, 1 × 108, 1 × 107 spores/mL) were prepared, every group infected 15 fourth instar larvae with 0.5 μL spore suspension (5 × 105, 5 × 104, 5 × 103 spores/larva) as describe above and each larva were kept in a 25 mL plastic cup. The cup and diet were changed daily, and frass was collected daily to check whether the microsporidia present under 400× light microscopy by fresh wet smears. The period from feeding spores to the first appearance of spores in frass is latent period [10,25]. The data were found to follow a normal distribution by the Shapiro–Wilk test. One-way ANOVA analysis and Tukey’s multiple comparisons test were used to check significance.

2.3. Ultra-Histopathology

Starved fourth instar larvae were inoculated with 5 × 105 spore/larva; after 4 days, infected and healthy midgut tissues were dissected and immediately fixed in 2.5% glutaraldehyde (pH 7.4) at 4 °C for 24 h. Tissues were rinsed in 0.2 M phosphate buffer and post-fixed in 1% osmium tetroxide (OsO4 in 0.2 M phosphate buffer) for 2 h at 4 °C, and dehydrated in 30%, 50%, 60%, 70%, 80%, 90%, 95%,100% ethanol, then embedded in epoxy resin. Ultrathin sections (80–100 nm) were taken with Leica EM UC7 (Leica Microsystems, Wetzlar, Germany), and stained with saturated uranyl acetate and Reynolds’ lead citrate. Samples were observed under a HITACHI HT7800 (Hitachi High-Tech Corporation, Tokyo, Japan) transmission electron microscope.

2.4. Impact of Nosema sp. on Development of S. frugiperda

Starved fourth instar larvae were inoculated with 5 × 105, 5 × 104, 5 × 103, and 0 spores/larva as described above; each treatment group was set up with 3 replicates and 30 individuals per replicate. The larvae were checked to determine whether dead twice a day, and the age of death and developmental duration of each instar were recorded. In each group, 30 larvae were randomly selected, and their body weights were recorded daily until death or until the 10th day (whichever occurred first). The data were found to follow a normal distribution by the Shapiro–Wilk test. One-way ANOVA analysis and Tukey’s multiple comparisons test were used to check significance.

2.5. RNA-Seq

Starved fourth instar larvae were inoculated with 5 × 105 spore/larva; after 4 days (24 h of 5th instar), total RNAs were extracted from healthy and infected larvae for constructing RNA sequencing libraries, and each treatment group was set up with 3 replicates and 3 individuals per replicate. The sequencing libraries were sequenced on the Illumina HiSeq 2000 platform by Beijing Tsingke Biotechnology Co., Ltd. (Beijing, China). Transcripts were annotated on the basis of the reference genome (http://v2.insectgenome.com/Organism/715, accessed on 3 April 2024). DESeq2 was used to analyze the differential expression of identified genes [26], and those with p < 0.05 and fold change ≥2 were considered to be significantly differentially expressed. Gene ontology (GO) enrichment and KEGG pathway analysis (https://www.genome.jp/kegg/, accessed on 10 April 2024) were used to identify the functional modules of differential expression genes.

2.6. Impact of Nosema sp. on Genes of Chitin Synthesis Pathway of S. frugiperda

Starved fourth instar larvae were inoculated with 5 × 105 spores/larva as described above. The larva at 12 h, 24 h, and 48 h of the fifth instar were collected, and total RNA was extracted by Trizol (TRIzol® Reagent, Ambion®, Thermo Fisher Scientific Inc., Waltham, MA, USA). Three larvae were taken at each time point, and three replicates were set up. The RNA quality and concentration were measured with a micro nucleic acid analyzer NanoDrop™ 2000 (Thermo Fisher Scientific Inc., Waltham, MA, USA). A total of 1 μg of RNA was reverse transcribed into cDNA according to instruction (TRUE script RT MasterMix, Aidlab Biotechnologies Co., Ltd., Beijing, China). The gene expression was detected with M5 HiPer SYBR Premix EsTaq plus (with Tli RNaseH) kit (Mei5 Biotechnology Co., Ltd., Beijing, China) in a Bio-Rad CFX Connect Real-Time System (Bio-Rad Laboratories Inc., Hercules, CA, USA). qPCR system: M5 HiPer SYBR Premix EsTaq plus 10 μL, forward primer 0.5 μL, reverse primer 0.5 μL, cDNA 1 μL, DNase/RNase-free water 8 μL. qPCR procedure: 95 °C for 30 s; 40 cycles of 95 °C for 5 s and 60 °C for 40 s; 95 °C for 10 s; melt curve at 60–95 °C. The genes related to chitin synthesis and housekeeping gene primers are shown in Table S1. Three biological and three technical replicates were set up. Moreover, 2−ΔΔCT method was used for data processing [27], and t-test was used for significance analysis. The data of the Infected group and the Control group were each put through the Shapiro–Wilk normality test, one-way ANOVA, and Tukey’s multiple comparisons test.

3. Results

3.1. Ultra-Histopathology Within Latent Period in S. frugiperda Infected by Nosema sp.

The periods were 6.53 ± 1.60 (n = 15), 8.00 ± 1.85 (n = 15), and 9.50 ± 1.51 (n = 10) (mean ± SD) days in 5 × 105, 5 × 104, and 5 × 103 spores/larva groups, respectively. One-way ANOVA analysis showed that inoculation dose significantly affected the latent period (F 2,37 = 9.5, p < 0.05), and there was a significant difference between 5 × 105 and 5 × 103 spores/larva groups (p = 0.0003) (Figure S1)
Ultrastructural analysis of midgut tissues from S. frugiperda larvae at 4 days post-microsporidian inoculation revealed distinct pathological alterations (Figure S2). The most prominent of these was the appearance of vacuoles within the cytoplasm located in close proximity to the mitochondria. And the mitochondria became thinner and longer, while the normal mitochondria are oval in shape. The mitochondria were observed to semienclose the spores, and it is hypothesized that this might be the reason for the elongation of the mitochondria. Vacuoles were also present in the intercellular spaces and mitochondria. Another obvious histological lesion was the detachment of goblet cells, and microvilli broke and filled the goblet cavity, while in normal circumstances, goblet cells adhere closely to columnar cells.

3.2. Impact of Developmental Duration, Weights, and Virulence on S. frugiperda Infected by Nosema sp.

The symptom of molting failure was identified as the primary cause of mortality, and the molt failure rates were 45.6%, 57.8%, and 31.5% in 5 × 105, 5 × 104, and 5 × 103 spores/larva groups, respectively (Figure 1A). Under different inoculation doses, the lethal age of microsporidia to S. frugiperda larvae was different. At the dose of 5 × 105 spores, a few individuals died at the 4th instar, and the larvae mainly died at the 5th and 6th instars. At the dose of 5 × 104 spores, individuals mainly died at the 5th, 6th, and 7th instars. And at the dose of 5 × 103 spores, the 6th and 7th larvae and pupae died mainly (Figure 1B). And the mortality in the larvae stage was 98.9%, 97.8%, and 64.0%, respectively, from high to low dose, and the median lethal time (LT50) was calculated to be approximately 14, 12, and 27.5 days, respectively, from high to low dose (Figure 1C).
The developmental duration is shown in Table 1. Larvae exhibited significantly prolonged developmental duration across all instars following microsporidia inoculation. Notably, infected larvae that succumbed during each respective instar showed significantly extended survival periods compared to their surviving individuals, except at the 5th instar infected with 5 × 103 spores (Figure 2).
The daily body weights of larvae were measured within 10 days after microsporidia infection when larvae were 4th instar. The results showed that within 4 days post-infection, there was no significant change in body weight among the treatment groups. On the 5th day, a significant difference emerged between the 5 × 105 group and the control group (p = 0.0004). On the 6th day, a significant difference was observed between the 5 × 104 group and the control group (p < 0.0001). On the 7th day, a significant difference occurred between the 5 × 103 group and the control group (p = 0.0059). Notably, there was no difference between the 5 × 105 group and the 5 × 104 group throughout the experiment, while a significant difference persisted between the 5 × 105 group and the 5 × 103 group starting from the 5th day. These findings indicate that microsporidia infection significantly affects the body weight of the host, and different inoculation doses also have a significant impact on the host’s body weight (Figure 3).

3.3. RNA-Seq Analysis

The main sequencing information of RNA-seq is shown in Table S2. Transcriptome analysis results indicated that S. frugiperda following microsporidian infection identified 3668 differentially expressed genes (DEGs), comprising 1791 upregulated and 1877 downregulated transcripts (Figure 4A). KEGG enrichment analysis revealed that the Amino sugar and nucleotide sugar metabolism pathway was one of the most significantly enriched pathways (Figure 4C). GO analysis demonstrated that the differentially expressed genes were predominantly concentrated in the category of Catalytic activity (Figure 4D). Notably, we found that genes encoding relevant enzymes in the hexosamine pathway of the chitin synthesis pathway were annotated in both the Amino sugar and nucleotide sugar metabolism pathway and the Catalytic activity category. Among these genes, GFAT (EC 2.6.1.16), GNPNA (EC 2.3.1.4), PAGM (EC 5.4.2.3), and UAP (EC 2.7.7.23) exhibited consistent downregulation, and CHS (EC 2.4.1.16) displayed bidirectional regulation (Figure 4E).

3.4. Gene Expression of Chitin Synthesis Pathway

The expression levels of all genes in the chitin synthesis pathway at three different time points in the 5th instar larvae of S. frugiperda were measured (Figure 5). Compared to uninfected counterparts, infected larvae exhibited significantly reduced expression of TRE1, G6PI, GFAT, GNPNA, and UAP genes at 12 h of 5th instar larvae. At 24 h, G6PI gene expression was significantly reduced in infected larvae, while TRE2 and CHS2 genes were significantly upregulated. And at 48 h post of 5th instar, infected larvae had significantly lower expression of GFAT, PAGM, and CHS1 genes. These results were generally consistent with the transcriptome analysis results. Additionally, significant temporal dynamics were observed in the expression of chitin synthesis pathway genes in uninfected larvae, but some genes in infected individuals showed no significant variations at different times (e.g., TRE1, G6PI, GFAT, GNPNA, PAGM). Notably, the expression of CHS1 decreased significantly over time, indicating that microsporidian infection may affect the expression levels of genes in the chitin synthesis pathway, ultimately disrupting the normal process of chitin synthesis. We hypothesize that this disruption contributes to the prolonged developmental duration and molting failure of infected S. frugiperda larvae.

4. Discussion

The latent period of a pathogen is the time between the invasion of the host and the first production of infectious units [28] or the time between the invasion of the host and the first appearance of symptoms [29]. In this article, the latent period of microsporidia ranged from 6 to 10 days, depending on inoculation doses. Symptom manifestation (e.g., weight loss and prolonged developmental duration) preceded the detection of infective spores. This phenomenon occurs because newly generated microsporidian spores do not immediately release into the environment post-host infection but instead continue propagating within the host body [10]. Consequently, pathological damage has already commenced during the latent period of microsporidian infection.
Following microsporidian infection in insects, particularly lepidopteran hosts, the midgut emerges as the primary target tissue. To enable direct visualization of cellular pathologies induced by microsporidian infection, we employed transmission electron microscopy (TEM) for histopathological analysis. The infection of the host by Nosema sp. within the latent period had already caused severe damage to the cells. The most obvious symptom observed was cytoplasmic vacuolization, a phenomenon previously documented in Nosema-infected hosts across multiple studies; however, this feature is not microsporidian-specific, as similar vacuolization patterns occur during Bacillus thuringiensis (Bt) infections [13,30]. Vacuoles appear around the mitochondria, and this phenomenon has also been confirmed in cells infected by Encephalitozoon microsporidia [31,32]. We have also observed some new pathological phenomena, such as the formation of vacuoles within mitochondria and the direct encapsulation of spores by mitochondria. Microsporidia lack mitochondria and need to obtain energy directly from the host [33]. The interaction between microsporidia and the host mitochondria that we have observed indicates that the energy source of microsporidia is the host mitochondria. The infection of host cells by Nosema sp. can also cause damage to goblet cells, such as the microvilli break; this can compromise ionic homeostasis and nutrient absorption, impairing physiological mechanisms of detoxification [34]. The insect midgut regulates growth and development through coordinated regulation of nutrient metabolism, hormonal signaling, and gut microbiota dynamics [35,36,37]. Therefore, Nosema sp. may inhibit the growth and development of the host by damaging the intestinal tissues.
Microsporidian infections are classified as chronic (slow-acting, progressing seriousness) or acute (fast-acting, short duration), depending on the microsporidian species, inoculation dose, and host instar at infection [10,12,38]. The latent period of microsporidian infection in 4th instar S. frugiperda larvae (approximately 5–9 days) was relatively long compared to the normal developmental duration from the 4th larval stage to pupation (approximately 12 days). And the characteristic manifestations of developmental retardation and gradual mortality post-infection align with the definition of chronic infection. However, we concurrently observed accelerated mortality in a minority of infected individuals, which may be attributed to compromised host immune competence. Thus, the manifestation of microsporidian infection in S. frugiperda as either chronic or acute infection is contingent upon the host’s physiological condition.
Chitin, an essential biopolymer in insects absent in plants and vertebrates, represents an ideal target for pest control strategies. Chitin synthase (CHS), the pivotal enzyme in chitin biosynthesis, plays a critical role in insect development [19]. In S. frugiperda, CHS1 exhibits predominant expression in the epidermis, and its silencing via SfCHS1-siRNA nanocomplex disrupts larval molting and pupation [39]. The chitin synthesis inhibitor 2,6-difluorobenzoylurea inhibits the expressions of TRE1, HK, G6PI, GFAT, and CHS1, resulting in the obstruction of molting in S. frugiperda and ultimately leading to its death [40]. Transcriptome analysis revealed widespread suppression of genes within the chitin biosynthesis pathway. qPCR validation demonstrated significant CHS1 downregulation in microsporidia-infected larvae at 48 h post-5th-instar. Concurrently, healthy larvae initiated molting preparations while infected counterparts exhibited complete molting arrest, suggesting microsporidia prolong larval development through targeted CHS1 suppression, thereby blocking ecdysis progression.
Notably, similar to the results of the transcriptome analysis, the expression level of CHS2 in the infected larvae was upregulated at 24 h post-5th instar. As CHS2 primarily functions in midgut peritrophic membrane formation [19], and our ultrastructural histopathology confirmed microsporidia-induced midgut cell damage, we speculate that the observed CHS2 upregulation may reflect a compensatory mechanism to repair peritrophic membrane lesions caused by infection, this hypothesis warrants further experimental validation. The expression pattern of TRE2 is similar to that of CHS2, indicating that TRE2 is related to the peritrophic membrane in S. frugiperda. The expression levels of other genes in the chitin synthesis pathway (including TRE1, G6PI, GFAT, GNPNA, PAGM, and UAP) were also inhibited after S. frugiperda was infected by Nosema sp. The inhibition of upstream genes in the chitin synthesis pathway also affects the growth and development of the host [41,42]. In addition, our results demonstrated genes of the chitin synthesis pathway exhibited dynamic expression patterns during normal larval development, but after microsporidia infection, the expression levels remained stable or were continuously inhibited, which may be one of the reasons for host developmental obstruction.

Supplementary Materials

The following supporting information can be downloaded at: https://www.mdpi.com/article/10.3390/microorganisms13050994/s1. Table S1: The primers for qPCR; Table S2: Sequencing information of RNA-seq; Figure S1: Latent period in S. frugiperda infected by Nosema sp.; Figure S2: Ultra-histopathology of the midgut of S. frugiperda infected by Nosema sp.

Author Contributions

Writing—original draft, Y.X.; writing—review and editing, W.S. and S.T.; methodology; Y.X., H.L., and X.H.; investigation, Y.X. and H.L.; formal analysis, Y.X.; visualization, Y.X.; resources, W.S.; funding acquisition, W.S. All authors have read and agreed to the published version of the manuscript.

Funding

This work was supported by the National Key Research and Development Program of China [2021YFD1400703].

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

The original contributions presented in this study are included in the article/Supplementary Material. Further inquiries can be directed to the corresponding authors.

Conflicts of Interest

The authors declare no conflicts of interest.

References

  1. Sun, X.X.; Hu, C.X.; Jia, H.R.; Wu, Q.L.; Shen, X.J.; Zhao, S.Y.; Jiang, Y.Y.; Wu, K.M. Case study on the first immigration of fall armyworm, Spodoptera frugiperda invading into China. J. Integr. Agric. 2021, 20, 664–672. [Google Scholar] [CrossRef]
  2. Makale, F.; Mugambi, I.; Kansiime, M.K.; Yuka, I.; Abang, M.; Lechina, B.S.; Rampeba, M.; Rwomushana, I. Fall armyworm in Botswana: Impacts, farmer management practices and implications for sustainable pest management. Pest Manag. Sci. 2022, 78, 1060–1070. [Google Scholar] [CrossRef]
  3. Wei, L.; Nei, Y.; Li, Y.J. Research progress on green and sustainable prevention and control technologies for Spodoptera frugiperda. Chin. J. Biol. Control. 2024; in press. [Google Scholar]
  4. Van den Berg, J.; du Plessis, H. Chemical Control and Insecticide Resistance in Spodoptera frugiperda (Lepidoptera: Noctuidae). J. Econ. Entomol. 2022, 115, 1761–1771. [Google Scholar] [CrossRef] [PubMed]
  5. Rivero-Borja, M.; Guzmán-Franco, A.W.; Rodríguez-Leyva, E.; Santillán-Ortega, C.; Pérez-Panduro, A. Interaction of Beauveria bassiana and Metarhizium anisopliae with chlorpyrifos ethyl and spinosad in Spodoptera frugiperda larvae. Pest Manag. Sci. 2018, 74, 2049–2056. [Google Scholar] [CrossRef]
  6. Dong, H.; Zhu, K.H.; Zhao, Q.; Bai, X.P.; Zhou, J.C.; Zhang, L.S. Morphological defense of the egg mass of Spodoptera frugiperda (Lepidoptera: Noctuidae) affects parasitic capacity and alters behaviors of egg parasitoid wasps. J. Asia-Pac. Entomol. 2021, 24, 671–678. [Google Scholar] [CrossRef]
  7. Stinguel, P.; Paiva, C.E.C.; Zuim, V.; Azevedo, A.C.T.; Valicente, F.H.; Santos Júnior, H.J.G. Optimization of in vivo production of Spodoptera frugiperda multiple nucleopolyhedrovirus (SfMNPV). Neotrop. Entomol. 2022, 51, 122–132. [Google Scholar] [CrossRef]
  8. Zhang, H.J.; Sun, X.L.; Hao, H.Y.; Liu, S.S.; Guo, N.; Shi, J. Identification and pathogenicity of an entomopathogenic microsporidium collected from fall armyworm Spodoptera frugiperda. J. Plant Prot. 2022, 49, 1513–1520. [Google Scholar]
  9. Han, B.; Weiss, L.M. Microsporidia: Obligate Intracellular Pathogens Within the Fungal Kingdom. Microbiol. Spectr. 2017, 5, 10–1128. [Google Scholar] [CrossRef]
  10. Weiss, L.M.; Becnel, J.J. Microsporidia: Pathogens of Opportunity; Wiley-Blackwell: Oxford, UK, 2014. [Google Scholar]
  11. Shi, W.; Guo, Y.; Xu, C.; Tan, S.; Miao, J.; Feng, Y.; Zhao, H.; St Leger, R.J.; and Fang, W. Unveiling the mechanism by which microsporidian parasites prevent locust swarm behavior. Proc. Natl. Acad. Sci. USA 2014, 111, 1343–1348. [Google Scholar] [CrossRef]
  12. Simões, R.A.; Feliciano, J.R.; Solter, L.F.; Delalibera, I. Impacts of Nosema sp. (Microsporidia: Nosematidae) on the sugarcane borer, Diatraea saccharalis (Lepidoptera: Crambidae). J. Invertebr. Pathol. 2015, 129, 7–12. [Google Scholar] [CrossRef]
  13. Kermani, N.; Abu-Hassan, Z.A.; Dieng, H.; Ismail, N.F.; Attia, M.; Ghani, I.A. Pathogenicity of Nosema sp. (Microsporidia) in the diamondback moth, Plutella xylostella (Lepidoptera: Plutellidae). PLoS ONE 2013, 8, e62884. [Google Scholar] [CrossRef] [PubMed]
  14. Li, T.; Fang, Z.; He, Q.; Wang, C.; Meng, X.; Yu, B.; Zhou, Z. Characterizing the xenoma of Vairimorpha necatrix provides insights into the most efficient mode of microsporidian proliferation. Front. Cell. Infect. Microbiol. 2021, 11, 699239. [Google Scholar]
  15. Szumowski, S.C.; Troemel, E.R. Microsporidia-host interactions. Curr. Opin. Microbiol. 2015, 26, 10–16. [Google Scholar] [CrossRef]
  16. Ma, Z.; Li, C.; Pan, G.; Li, Z.; Han, B.; Xu, J.; Lan, X.; Chen, J.; Yang, D.; Chen, Q.; et al. Genome-wide transcriptional response of silkworm (Bombyx mori) to infection by the microsporidian Nosema bombycis. PLoS ONE 2013, 8, e84137. [Google Scholar] [CrossRef] [PubMed]
  17. Martín-Hernández, R.; Higes, M.; Sagastume, S.; Juarranz, Á.; Dias-Almeida, J.; Budge, G.E.; Meana, A.; Boonham, N. Microsporidia infection impacts the host cell’s cycle and reduces host cell apoptosis. PLoS ONE 2017, 12, e0170183. [Google Scholar] [CrossRef]
  18. Lopez-Ezquerra, A.; Mitschke, A.; Bornberg-Bauer, E.; Joop, G. Tribolium castaneum gene expression changes after Paranosema whitei infection. J. Invertebr. Pathol. 2018, 153, 92–98. [Google Scholar] [CrossRef]
  19. Yu, A.; Beck, M.; Merzendorfer, H.; Yang, Q. Advances in understanding insect chitin biosynthesis. Insect Biochem. Mol. Biol. 2024, 164, 104058. [Google Scholar] [CrossRef]
  20. Yao, Q.; Quan, L.F.; Xu, S.; Dong, Y.Z.; Li, W.J.; Chen, B.X. Effect of diflubenzuron on the chitin biosynthesis pathway in Conopomorpha sinensis eggs. Insect Sci. 2021, 28, 1061–1075. [Google Scholar] [CrossRef]
  21. Zhu, K.Y.; Merzendorfer, H.; Zhang, W.; Zhang, J.; Muthukrishnan, S. Biosynthesis, turnover, and functions of chitin in insects. Annu. Rev. Entomol. 2016, 61, 177–196. [Google Scholar] [CrossRef]
  22. Chen, J.; Tang, B.; Chen, H.; Yao, Q.; Huang, X.; Chen, J.; Zhang, D.; Zhang, W. Different functions of the insect soluble and membrane-bound trehalase genes in chitin biosynthesis revealed by RNA interference. PLoS ONE 2010, 5, e10133. [Google Scholar] [CrossRef]
  23. Pearson, J.C.; Juarez, M.T.; Kim, M.; Drivenes, Ø.; McGinnis, W. Multiple transcription factor codes activate epidermal wound-response genes in Drosophila. Proc. Natl. Acad. Sci. USA 2009, 106, 2224–2229. [Google Scholar] [CrossRef]
  24. Johny, S.; Kanginakudru, S.; Muralirangan, M.C.; Nagaraju, J. Morphological and molecular characterization of a new microsporidian (Protozoa: Microsporidia) isolated from Spodoptera litura (Fabricius) (Lepidoptera: Noctuidae). Parasitology 2006, 132, 803–814. [Google Scholar] [CrossRef]
  25. Hopper, J.V.; Mills, N.J. Pathogenicity, prevalence and intensity of a microsporidian infection by Nosema fumiferanae postvittana in the light brown apple moth, Epiphyas postvittana, in California. J. Invertebr. Pathol. 2016, 134, 27–34. [Google Scholar] [CrossRef] [PubMed]
  26. Love, M.I.; Huber, W.; Anders, S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 2014, 15, 550. [Google Scholar] [CrossRef] [PubMed]
  27. Livak, K.J.; Schmittgen, T.D. Analysis of relative gene expression data using real-time quantitative PCR and the 2−ΔΔCT method. Methods 2001, 25, 402–408. [Google Scholar] [CrossRef] [PubMed]
  28. Anderson, R.M.; May, R.M. Infectious Diseases of Humans: Dynamics and Control; Oxford University Press: Oxford, UK, 1992. [Google Scholar]
  29. Pu, Z.L. Insect Pathology; Guangdong Science and Technology Press: Guangdong, China, 1994. [Google Scholar]
  30. Wiwat, C.; Thaithanun, S.; Pantuwatana, S.; Bhumiratana, A. Toxicity of chitinase-producing Bacillus thuringiensis ssp. kurstaki HD-1 (G) toward Plutella xylostella. J. Invertebr. Pathol. 2000, 76, 270–277. [Google Scholar] [CrossRef]
  31. Scanlon, M.; Leitch, G.J.; Visvesvara, G.S.; Shaw, A.P. Relationship between the host cell mitochondria and the parasitophorous vacuole in cells infected with Encephalitozoon microsporidia. J. Eukaryot. Microbiol. 2004, 51, 81–87. [Google Scholar] [CrossRef]
  32. Han, B.; Ma, Y.; Tu, V.; Tomita, T.; Mayoral, J.; Williams, T.; Horta, A.; Huang, H.; Weiss, L.M. Microsporidia interact with host cell mitochondria via voltage-dependent anion channels using sporoplasm surface protein 1. mBio 2019, 10, e01944-19. [Google Scholar] [CrossRef]
  33. Solter, L.E.; Becnel, J.J.; Oi, D.H. Microsporidian entomopathogens. In Insect Pathology; Vega, F.E., Kaya, H.K., Eds.; Academic Press: San Diego, CA, USA, 2012; pp. 221–263. [Google Scholar]
  34. Castro, B.M.C.E.; Martínez, L.C.; Plata-Rueda, A.; Soares, M.A.; Tavares, W.S.; Serrão, J.E.; Zanuncio, J.C. Chlorantraniliprole degenerates microvilli goblet cells of the Anticarsia gemmatalis (Lepidoptera: Noctuidae) midgut. Chemosphere 2019, 229, 525–528. [Google Scholar] [CrossRef]
  35. Engel, P.; Moran, N.A. The gut microbiota of insects—Diversity in structure and function. FEMS Microbiol. Rev. 2013, 37, 699–735. [Google Scholar] [CrossRef]
  36. Shuttleworth, L.A.; Khan, M.A.M.; Osborne, T.; Collins, D.; Srivastava, M.; Reynolds, O.L. A walk on the wild side: Gut bacteria fed to mass-reared larvae of Queensland fruit fly [Bactrocera tryoni (Froggatt)] influence development. BMC Biotechnol. 2019, 19 (Suppl. S2), 95. [Google Scholar] [CrossRef] [PubMed]
  37. Wu, K.; Li, S.; Wang, J.; Ni, Y.; Huang, W.; Liu, Q.; Ling, E. Peptide hormones in the insect midgut. Front. Physiol. 2020, 11, 191. [Google Scholar] [CrossRef] [PubMed]
  38. Myung-Sae, H.; Hitoshi, W. Transovarial transmission of two microsporidia in the silkworm, Bombyx mori, and disease occurrence in the progeny population. J. Invertebr. Pathol. 1988, 51, 41. [Google Scholar]
  39. Gong, C.; Hasnain, A.; Wang, Q.; Liu, D.; Xu, Z.; Zhan, X.; Liu, X.; Pu, J.; Sun, M.; Wang, X. Eco-friendly deacetylated chitosan base siRNA biological-nanopesticide loading cyromazine for efficiently controlling Spodoptera frugiperda. Int. J. Biol. Macromol. 2023, 241, 124575. [Google Scholar] [CrossRef]
  40. Chen, J.P.; Xie, J.; Zhao, K.; Hu, Z.; Zhang, X.; Nan, X.H.; Sun, R.F. Effects of a novel 2,6-difluorobenzoylurea compound on the bioactivity and chitin synthesis of Spodoptera frugiperda. Chin. J. Pestic. Sci. 2023, 25, 798–807. [Google Scholar]
  41. Zou, H.; Zhang, B.; Zou, C.; Ma, W.; Zhang, S.; Wang, Z.; Bi, B.; Li, S.; Gao, J.; Zhang, C.; et al. Knockdown of GFAT disrupts chitin synthesis in Hyphantria cunea larvae. Pestic. Biochem. Physiol. 2022, 188, 105245. [Google Scholar] [CrossRef]
  42. Zhou, Y.J.; Du, J.; Li, S.W.; Shakeel, M.; Li, J.J.; Meng, X.G. Cloning, characterization, and RNA interference effect of the UDP-N-acetylglucosamine pyrophosphorylase gene in Cnaphalocrocis medinalis. Genes 2021, 12, 464. [Google Scholar] [CrossRef]
Microorganisms 13 00994 g001
Figure 1. (A): The molt failure rate in different instar stages and the symptom of molt failure; (B): the proportion of deaths at different instar stages after the 4th instar larvae were infected by Nosema sp.; (C): survival curves of S. frugiperda infected by Nosema sp. at different dosages.
Figure 1. (A): The molt failure rate in different instar stages and the symptom of molt failure; (B): the proportion of deaths at different instar stages after the 4th instar larvae were infected by Nosema sp.; (C): survival curves of S. frugiperda infected by Nosema sp. at different dosages.
Microorganisms 13 00994 g001
Microorganisms 13 00994 g002
Figure 2. The developmental duration of S. frugiperda larvae under different inoculation doses of Nosema sp. Letters represent the results of One-way ANOVA analysis and Tukey’s multiple comparisons among uninfected individuals, infected surviving individuals, and infected dead individuals at the same instar stage (p < 0.05). The absence of columns represents that n < 3, which is not included in the statistics.
Figure 2. The developmental duration of S. frugiperda larvae under different inoculation doses of Nosema sp. Letters represent the results of One-way ANOVA analysis and Tukey’s multiple comparisons among uninfected individuals, infected surviving individuals, and infected dead individuals at the same instar stage (p < 0.05). The absence of columns represents that n < 3, which is not included in the statistics.
Microorganisms 13 00994 g002
Microorganisms 13 00994 g003
Figure 3. The daily body weight of S. frugiperda after being infected by Nosema sp. Letters represent the results of One-way ANOVA and Tukey’s multiple comparisons among different treatment groups at the same time point (p < 0.05).
Figure 3. The daily body weight of S. frugiperda after being infected by Nosema sp. Letters represent the results of One-way ANOVA and Tukey’s multiple comparisons among different treatment groups at the same time point (p < 0.05).
Microorganisms 13 00994 g003
Microorganisms 13 00994 g004
Figure 4. Transcriptome analysis of DEGs between the healthy and Nosema sp. infected S. frugiperda. (A): Volcano plots showing the DEGs between the healthy and Nosema sp. infected S. frugiperda, red dots represent upregulated genes in infected group, green dots represent downregulated genes in infected group, and black dots indicate genes with no significant differences. (B): Heatmap of DEGs. Blue represents a lower level of expression, while red represents a higher level of expression. (C): KEGG pathway enrichment. (D): GO enrichment (Molecular Function). (E): KEGG map. Chitin synthesis pathway (Starting from Fru-6P, they are GlcN-6P, GlcNAc-6P, GlcNAc-1P, UDP-GlcNAc, and Chitin in sequence) in Amino sugar and nucleotide sugar metabolism pathway (ko00520). Green represents downregulated genes, and blue represents the genes upregulate and downregulate.
Figure 4. Transcriptome analysis of DEGs between the healthy and Nosema sp. infected S. frugiperda. (A): Volcano plots showing the DEGs between the healthy and Nosema sp. infected S. frugiperda, red dots represent upregulated genes in infected group, green dots represent downregulated genes in infected group, and black dots indicate genes with no significant differences. (B): Heatmap of DEGs. Blue represents a lower level of expression, while red represents a higher level of expression. (C): KEGG pathway enrichment. (D): GO enrichment (Molecular Function). (E): KEGG map. Chitin synthesis pathway (Starting from Fru-6P, they are GlcN-6P, GlcNAc-6P, GlcNAc-1P, UDP-GlcNAc, and Chitin in sequence) in Amino sugar and nucleotide sugar metabolism pathway (ko00520). Green represents downregulated genes, and blue represents the genes upregulate and downregulate.
Microorganisms 13 00994 g004
Microorganisms 13 00994 g005
Figure 5. Gene expression of chitin synthesis in 5th instar S. frugiperda at different times. The bar showed SE, “*” represents significant differences between CK and Infect group (t-test, p < 0.05). Uppercase and lowercase letters represent significant temporal variations in gene expression within control and infected groups, respectively (One-way ANOVA Analysis and Tukey’s multiple comparisons, p < 0.05).
Figure 5. Gene expression of chitin synthesis in 5th instar S. frugiperda at different times. The bar showed SE, “*” represents significant differences between CK and Infect group (t-test, p < 0.05). Uppercase and lowercase letters represent significant temporal variations in gene expression within control and infected groups, respectively (One-way ANOVA Analysis and Tukey’s multiple comparisons, p < 0.05).
Microorganisms 13 00994 g005
Table 1. The developmental durations (days) of surviving and dead individuals at each instar stage in 4th instar larvae under different inoculation doses.
Table 1. The developmental durations (days) of surviving and dead individuals at each instar stage in 4th instar larvae under different inoculation doses.
ck5 × 1055 × 1045 × 103
InstarAliveAliveDeadAliveDeadAliveDead
4th2.44 ± 0.32
n = 90		3.36 ± 1.53
n = 85		5.80 ± 1.48
n = 5		2.70 ± 0.35
n = 90		/2.58 ± 0.23
n = 89		/
5th2.54 ± 0.40
n = 90		5.03 ± 1.20
n = 38		8.53 ± 4.39
n = 47		4.75 ± 1.85
n = 48		7.77 ± 2.50
n = 42		3.31 ± 1.03
n = 83		3.67 ± 1.50
n = 6
6th2.88 ± 0.50
n = 90		5.33 ± 1.35
n = 9		11.16 ± 5.93
n = 29		4.80 ± 1.50
n = 20		7.85 ± 5.00
n = 27		3.77 ± 1.38
n = 52		5.90 ± 3.05
n = 31
7th5.66 ± 0.80
n = 88		/11.81 ± 2.95
n = 9		/13.58 ± 4.83
n = 25		7.53 ± 1.51
n = 33		15.50 ± 4.29
n = 19
Mean ± SD, “/” indicates that n < 3, and these data are not included in the statistics.
Disclaimer/Publisher’s Note: The statements, opinions and data contained in all publications are solely those of the individual author(s) and contributor(s) and not of MDPI and/or the editor(s). MDPI and/or the editor(s) disclaim responsibility for any injury to people or property resulting from any ideas, methods, instructions or products referred to in the content.

Share and Cite

MDPI and ACS Style

Xu, Y.; Liu, H.; Huang, X.; Tan, S.; Shi, W. The Developmental Disorders of Fall Armyworm (Spodoptera frugiperda, Lepidoptera: Noctuidae) Caused by the Infection with Nosema sp. (Microsporidia: Nosematidae). Microorganisms 2025, 13, 994. https://doi.org/10.3390/microorganisms13050994

AMA Style

Xu Y, Liu H, Huang X, Tan S, Shi W. The Developmental Disorders of Fall Armyworm (Spodoptera frugiperda, Lepidoptera: Noctuidae) Caused by the Infection with Nosema sp. (Microsporidia: Nosematidae). Microorganisms. 2025; 13(5):994. https://doi.org/10.3390/microorganisms13050994

Chicago/Turabian Style

Xu, Yudi, Haoyu Liu, Xinzheng Huang, Shuqian Tan, and Wangpeng Shi. 2025. "The Developmental Disorders of Fall Armyworm (Spodoptera frugiperda, Lepidoptera: Noctuidae) Caused by the Infection with Nosema sp. (Microsporidia: Nosematidae)" Microorganisms 13, no. 5: 994. https://doi.org/10.3390/microorganisms13050994

APA Style

Xu, Y., Liu, H., Huang, X., Tan, S., & Shi, W. (2025). The Developmental Disorders of Fall Armyworm (Spodoptera frugiperda, Lepidoptera: Noctuidae) Caused by the Infection with Nosema sp. (Microsporidia: Nosematidae). Microorganisms, 13(5), 994. https://doi.org/10.3390/microorganisms13050994

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop