Next Article in Journal
Mealybug Population Dynamics: A Comparative Analysis of Sampling Methods for Saccharicoccus sacchari and Heliococcus summervillei in Sugarcane (Saccharum sp. Hybrids)
Previous Article in Journal
The Potential Implications of Sex-Specific Differences in the Intestinal Bacteria of the Overwintering Wolf Spider Pardosa astrigera (Araneae: Lycosidae)
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Insects
Volume 15
Issue 7
10.3390/insects15070491
insects-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 thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Review

The Biological Roles of microRNAs in Drosophila Development

by
Daegyu Jang
†,
Chae Jeong Kim
†,
Bo Hyun Shin
† and
Do-Hwan Lim
*
School of Systems Biomedical Science, Soongsil University, Seoul 06978, Republic of Korea
*
Author to whom correspondence should be addressed.
†
These authors contributed equally to this work.
Insects 2024, 15(7), 491; https://doi.org/10.3390/insects15070491
Submission received: 23 May 2024 / Revised: 24 June 2024 / Accepted: 27 June 2024 / Published: 30 June 2024
(This article belongs to the Special Issue Research on Insect Epigenetics)
Browse Figures
Versions Notes

Abstract

:

Simple Summary

Drosophila (or the fruit fly) is widely used to study developmental processes associated with gene regulation. Insect development, including that of Drosophila, is controlled by various gene regulation mechanisms. In particular, numerous studies on microRNAs (miRNAs) in Drosophila have highlighted their crucial roles in development. This review focuses on the function of miRNAs in various tissues and developmental processes in Drosophila, along with sequencing technologies for studying miRNA interactions with target genes.

Abstract

Drosophila is a well-established insect model system for studying various physiological phenomena and developmental processes, with a focus on gene regulation. Drosophila development is controlled by programmed regulatory mechanisms specific to individual tissues. When key developmental processes are shared among various insects, the associated regulatory networks are believed to be conserved across insects. Thus, studies of developmental regulation in Drosophila have substantially contributed to our understanding of insect development. Over the past two decades, studies on microRNAs (miRNAs) in Drosophila have revealed their crucial regulatory roles in various developmental processes. This review focuses on the biological roles of miRNAs in specific tissues and processes associated with Drosophila development. Additionally, as a future direction, we discuss sequencing technologies that can analyze the interactions between miRNAs and their target genes, with the aim of enhancing miRNA studies in Drosophila development.

1. Introduction

Development is a delicate process controlled by a variety of external and internal factors. These factors ultimately influence the temporal and spatial regulation of genes involved in various developmental processes. Gene expression is regulated in two steps, namely transcription and post-transcription. Various transcription factors control the expression of numerous genes, orchestrating intrinsic cellular programs for proper development. Subsequently, after transcription, individual RNAs can be regulated by diverse mechanisms, including suppression mediated by small non-coding RNAs called microRNAs (miRNAs) [1].
Drosophila serves as an attractive insect model system for scientists studying developmental processes regulated by various gene regulatory mechanisms. This is because a combination of classical genetics with a variety of molecular, cellular, and biochemical techniques can be easily employed to study Drosophila development. The generation time of Drosophila from fertilized eggs to adult flies is approximately 10 days [2]. During this period, Drosophila, a holometabolous insect, undergoes four stages, namely embryonic, larval, pupal, and adult stages of development [2]. At each stage, individual cells differentiate into specific cell types and form distinct tissues under programmed signals. This review focuses on developmental processes regulated by miRNAs.
Given that gene regulation mechanisms are important in the development of insects, including Drosophila, it is not surprising that miRNAs controlling gene expression have emerged as central regulators of development. Since the discovery that lin-4 plays a role in controlling the temporal development of Caenorhabditis elegans by negatively regulating lin-14 [3,4], efforts have been made to identify miRNAs generated from Drosophila using molecular biology and biochemistry techniques [5]. In the study, 16 miRNAs, including miR-1, miR-2b, and miR-6, were identified in Drosophila and S2 cells using a cloning method employing adapter ligation. The study also analyzed the expression patterns of these miRNAs at several developmental stages, including embryos, larvae, pupae, and adults. Some of the discovered miRNAs, such as miR-13a and miR-13b-1, were clustered. Through further efforts employing small RNA cloning, a non-redundant set of 62 miRNAs, including miR-34, miR-92a, and miR-184, was identified across various developmental stages, with the expression profiling of individual miRNAs [6]. In this study, the miR* sequences, which represent the opposite strand of the identified primary strand of miRNAs, were also cloned for some miRNAs (miR-10*, miR-13a*, and miR-281-2*), despite being relatively less abundant.
Subsequent studies employing computational approaches and high-throughput sequencing technologies led to the discovery of many novel miRNAs, including those with low expression levels [7,8]. According to the miRBase an miRNA database, 469 mature miRNAs have been identified in Drosophila melanogaster to date [9]. Despite the discovery of several hundred miRNAs in Drosophila, studies of their biological roles in developmental processes are limited.
The knowledge of known gene regulatory roles of miRNAs in development should be comprehensively summarized and shared with researchers in this field. A previous insightful review explained the biological roles of some known miRNAs in various developmental processes [10]. Additionally, a more recent review focused on miRNAs involved in embryonic development and specific developmental aspects, such as muscle development and homeotic gene regulation [11]. In this review, with recent additional results, we summarize the basic miRNA pathways in Drosophila and the known biological roles of miRNAs in relatively well-explored tissues, such as the nervous system, wing, and eye, as well as in processes associated with development, such as growth and cell death. Rather than attempting to cover all related literature on development-associated miRNAs, we focus on these specific areas. Additionally, we briefly discuss recent sequencing techniques that can be used to enhance our understanding of the regulatory function of miRNAs in Drosophila.

2. miRNA Biogenesis and Mechanism in Drosophila

The miRNA genes are encoded in the genome and transcribed by RNA polymerase II (Figure 1) [12]. As features of RNAs transcribed by RNA polymerase II, the resulting primary transcripts, known as primary miRNAs (pri-miRNAs), contain 5′ 7-methyl caps and 3′ poly-A tails [13]. These pri-miRNAs can be transcribed by several kilobases and often encompass multiple distinct miRNAs in clustered miRNA sets. A minor group of miRNAs is alternately transcribed by RNA polymerase III [14].
Pri-miRNAs, which contain stem–loop structures, undergo processing into precursor miRNAs (pre-miRNAs) of approximately 70 nucleotides (nt) in length. This process occurs via the endonucleolytic cleavage of the stem of the hairpin structure [15]. The cleavage process is catalyzed by the microprocessor complex comprising Drosha, a nuclear ribonuclease III (RNase III), and the Partner of Drosha (Pasha) in Drosophila (DGCR8 in humans) [16,17,18]. The cropping of pre-miRNAs from pri-miRNAs by Drosha occurs in a co-transcriptional manner [19]. However, a distinct type of miRNA known as mirtron, which bypasses the Drosha-mediated cleavage step, has been identified through high-throughput sequencing analysis in Drosophila [20,21]. Without Drosha processing, these mirtrons are processed into lariat mirtrons by spliceosomal machinery. Subsequently, they form structural mimics of the pre-miRNAs via a debranching process.
Cleaved pre-miRNAs exhibit high affinity for Ranbp21 (known as exportin 5 in humans) and are subsequently exported from the nucleus to the cytoplasm through the pre-miRNA–Ranbp21 interaction [22,23,24]. Depletion of Ranbp21 inhibits the export of pre-miRNAs, resulting in a reduction in mature miRNAs [22].
Pre-miRNAs are further processed into approximately 21 nt miRNA duplexes by the RNase III enzyme, Dicer (Dcr), in the cytoplasm [25,26,27]. In Drosophila, there are two Dcr proteins, Dcr-1 and Dcr-2, which play distinct roles [28]. Dcr-1 and Dcr-2 function in miRNA and siRNA pathways, respectively. Dcr recognizes the 2 nt 3′ overhang of pre-miRNAs using its PAZ domain and subsequently cleaves the stem of pre-miRNAs approximately 20 nt away [29,30]. This cleavage process yields an miRNA duplex.
These miRNA duplexes facilitate mRNA repression through an effector complex known as the miRNA-induced silencing complex (miRISC) [31]. The core protein within the miRISC is the Ago protein. In Drosophila, similar to Dcr, Ago1 and Ago2 are closely associated with miRNA and siRNA pathways, respectively [32,33]. Upon incorporation of the miRNA duplexes into Ago1, the two strands of the miRNA duplexes are dissociated, and eventually, one strand of the miRNA duplex, serving as the guide, is retained within the miRISC [34,35]. The strand of the miRNA incorporated into Ago1 is named with a −5p or −3p suffix, depending on whether it is generated from the 5′ or 3′ arm of the stem region in the pre-miRNA [36].
miRNAs generally bind to the 3′-untranslated region (3′-UTR) of target mRNAs in a sequence-specific manner, ultimately resulting in the inhibition of gene expression by suppressing translation and/or promoting mRNA decay [1].

3. Regulation of miRNA Expression by Hormones in Drosophila

Drosophila hormones regulate development. Among these, two essential hormones, ecdysteroids and juvenile hormones (JHs), are closely associated with the control of developmental timing and processes.
JH is produced by the corpus allatum of the ring gland [37]. Initially, JHs bind to methoprene-tolerant (Met) or germ cell-expressing JH intracellular receptors [38]. Met forms a complex with Taiman (Tai) and heat shock protein 83 (Hsp83) [39,40], and subsequently, Nucleoporin 358 kD (Nup358) facilitates the translocation of this complex into the nucleus [41]. This JH-Met complex binds to the JH response region and activates the expression of JH-responsive genes such as zinc-finger TF Krüppel-homolog 1 (Kr-h1) [37].
Ecdysone is released from the prothoracic glands of the ring gland [42]. Canonical ecdysone signaling is initiated by the binding of the active ecdysone metabolite, 20-hydroxyecdysone (20E), to a heterodimeric receptor comprising an ecdysone receptor (EcR) and ultraspiracle (USP) [43,44,45]. This complex directly activates the expression of a small set of primary response genes, such as broad (br), ecdysone-induced protein 74EF (E74), and ecdysone-induced protein 75EF (E75) [46,47,48]. These early ecdysone-responsive transcription factors then regulate a large set of secondary response genes encompassing both protein-coding and non-coding genes [49,50].
These hormone-signaling pathways regulate the expression of miRNAs that serve as central gene regulators, in addition to the regulating protein-coding genes. The dynamic expression of miRNAs, influenced by hormones, can lead to drastic alterations in the expression of various genes, such as those observed during metamorphosis [50,51], or fine-tune the expression of individual genes, as seen in differentiation processes.
Some research groups have identified miRNAs that respond to the titration of each hormone and are associated with developmental stages highly influenced by specific hormone activities. In the early stages of miRNA discovery in Drosophila, Lorenzo et al. found that miR-100, miR-125, and let-7, which are upregulated during the larval-to-pupal transition, also show increased expression in response to ecdysone hormones in S2 cells, as determined by northern blotting [52]. These three miRNAs (let-7-Complex, let-7-C) are co-transcribed and involved in normal adult behaviors through the regulation of remodeling of the abdominal neuromusculature [53]. In contrast, miR-34 expression was lower in 20E-treated S2 cells compared with that in untreated control cells. A study using cross-linking immunoprecipitation with deep sequencing (CLIP-seq) revealed that 30 Ago1-associated miRNAs (including miR-252-5p, miR-276a-3p/5p, and miR-279-3p) were upregulated, while 42 Ago1-associated miRNAs (including miR-317-3p and miR-8-5p) were downregulated following 20E treatment in S2 cells [50]. In another study using small RNA sequencing, 43 upregulated miRNAs (including miR-278-3p/5p, miR-306-5p, and miR-13a-3p) and 35 downregulated miRNAs (including miR-970-5p, miR-979-3p, and miR-998-3p) were identified in S2 cells treated with 20-hydroxyecdysone [54].
In addition to ecdysone-responsive miRNAs, Lorenzo et al. identified miR-34 as a JH-responsive miRNA in S2 cells [52]. Other studies found that the expression of miR-927, let-7, miR-100, and miR-125 is repressed in S2 cells by methoprene, a JH analog [55,56,57]. However, relatively few studies have been conducted on JH-responsive miRNAs compared with those on ecdysone-responsive miRNAs.

4. Biological Roles of miRNAs in Drosophila Development

A set of miRNAs is regulated by programmed signals, which subsequently affect various target genes involved in developmental processes. Here, we discuss the developmental processes in which the roles of miRNAs have been relatively well explored and review the functions of these miRNAs (Table 1).

4.1. Developmental Growth and Apoptosis

Proper regulation of growth and programmed cell death, including apoptosis, at each developmental stage is crucial for the developmental process. To date, many research studies have unveiled several miRNAs associated with these biological processes.

4.1.1. miRNAs Involved in Developmental Growth

According to previous observations, miRNAs upregulated by the ecdysone signaling pathway are typically associated with negative regulation of growth, whereas downregulated miRNAs are likely involved in positive regulation of growth.
Ecdysone-induced miRNA, miR-252, is expressed and functions in the fat body during the larval stage [50,58]. A lack of miR-252 leads to increased body weight in adult flies, while overexpression of miR-252 in the fat body results in a significant reduction in developmental growth, accompanied by a lower cell number and smaller cell size. Growth alteration upon the change in miR-252 expression is mediated by targeting mushroom bodies tiny (mbt), which encodes a p21-activated kinase. Additionally, miR-252 controls the cell cycle by regulating cyclins A and B by suppressing Abelson interacting protein (Abi) [50]. This also affects the developmental growth of Drosophila.
In addition to cell cycle control, the insulin/insulin-like growth factor signaling (IIS) pathway plays a central role in developmental growth in Drosophila. The IIS pathway is activated by the binding of Drosophila insulin-like peptides (dILPs) to Insulin-like receptors (InRs) (Figure 2A) [83]. In Drosophila, eight dILPs (dILPs 1-8) have been identified and are expressed in insulin-producing cells in the brain, visceral muscles of the gut, and fat body. Through the binding of dILPs to InR in the target tissues, docking proteins Chico (IRS fly ortholog) and Lnk (fly ortholog of SH2B adaptor proteins) were recruited [84]. Chico phosphorylates phosphoinositide-3 kinase (PI3K), transferring the signaling to phosphoinositide-dependent kinase 1 (PDK1) and Akt kinase (Akt1). Subsequently, this signaling pathway expands to the forkhead box—subgroup O (FOXO), shaggy (sgg), or Tsc1/Tsc2 complex [84]. This signaling cascade significantly impacts the developmental growth of Drosophila.
miR-276a, another ecdysone-induced miRNA, is also expressed in larval fat bodies [60]. When miR-276a is upregulated in the fat body, the total mass of the larval fat body is dramatically reduced, resulting in developmental growth defects. This defect is associated with the inactivation of insulin signaling by miR-276a-3p-mediated suppression of InR (Figure 2A). In contrast, miR-8, which is downregulated by ecdysone signaling, is implicated in the inhibition of the IIS pathway [62]. Deletion of miR-8 in flies results in a small body size with inactive IIS in the fat body. This phenotype is linked to the PI3K inhibitor-encoding u-shaped (ush), which is a target of miR-8 (Figure 2A). Moreover, miR-14 is downregulated by ecdysone signaling and controls the production of dILPs in insulin-producing neurosecretory cells [64,85]. Mutants lacking miR-14 show decreased dILP3 and dILP5 production. Regulation by miR-14 is achieved by targeting sugarbabe (sug) (Figure 2A).

4.1.2. miRNAs Involved in Programmed Cell Death

Programmed cell death, including apoptosis, is closely associated with Drosophila development. In Drosophila, various apoptotic stimuli induce the transcriptional expression of reaper-family genes, including reaper (rpr), head involution defective (hid), and grim (Figure 2B) [86]. These proteins can act as antagonizing inhibitors of Drosophila IAP-1 (Diap1), which functions as an E3-ubiquitin ligase, promoting the degradation of the initiator caspase, death regulator Nedd2-like caspase (Dronc) [86]. Dronc is activated by the Dark apoptosome and subsequently transduces apoptotic signals by cleaving and activating the effector caspases, namely Death related ICE-like caspase (Drice) and death caspase-1 (Dcp-1) [87].
Bantam miRNA was identified as an miRNA that promotes cell proliferation [66]. Analysis using an miRNA sensor revealed that Bantam activity was correlated with cell proliferation in the developing larval brain and wing discs. Bantam miRNA negatively regulates the expression of hid, resulting in the inhibition of hid-mediated apoptosis in Drosophila (Figure 2B) [66].
Additionally, miR-14 suppresses Drosophila cell death [65]. Reduced miR-14 activity leads to severe eye defects induced by Rpr. Conversely, eye-specific expression of miR-14 alleviates retinal cell death induced by Rpr, Hid, Grim, and Dronc [65]. The anti-apoptotic effect of miR-14 is likely achieved by regulating the levels of Drice (Figure 2B).
Furthermore, miR-6 and miR-11 are involved in the development of the embryonic central nervous system (CNS) through the regulation of the pro-apoptotic genes rpr, hid, grim, and sickle (skl) (Figure 2B) [68]. Recently, screening for anti-apoptotic miRNAs was performed in a Drosophila eye model induced by the misexpression of pro-apoptotic genes such as hid and grim [88]. From the screening, 16 miRNAs, including miR-7 and miR-125, were identified as apoptosis suppressors in both the GMR-hid and GMR-grim genetic backgrounds.

4.2. miRNAs in the Development of the Nervous System

Studies have revealed that miRNAs play important roles in the development of the nervous system in Drosophila. These miRNAs influence various developmental processes in the nervous system, including the growth, differentiation, structural formation, and maintenance of nerve cells, by regulating specific target genes in distinct cell types.

4.2.1. miR-92a/b, Bantam, and miR-124 in Neuroblasts (NBs)

The Drosophila nervous system is derived from neural stem cells known as NBs [89]. These NBs undergo asymmetric cell division to generate different neuronal subtypes. The self-renewal, differentiation, and proliferation of NBs are regulated by intrinsic gene regulatory programs, including miRNAs.
Both miR-92a and miR-92b are highly expressed in the NBs of the Drosophila larval brain [72]. miR-92a is located in the first intron of Jing interacting gene regulatory 1 (jigr1), while miR-92b is in the 3′-UTR downstream of the jigr1 coding region. Consequently, these two miRNAs are co-expressed with jigr1. In miR-92a/b knockout mutant flies, the number of NBs is significantly reduced. However, this reduction is not linked to an increase in apoptosis or defects in asymmetric cell division [72]. Instead, the loss of miR-92a/b leads to premature differentiation and reduced proliferation of neuroblasts. Due to these defects, miR-92a/b mutant flies exhibit a smaller ventral nerve cord and brain compared to control flies. MiR-92a/b negatively regulates the host gene, jigr1. Similarly, overexpression of jirg1 in NBs also results in a reduction in the brain size of adult flies due to the premature differentiation of NBs [72].
Bantam has been detected in the neuronal progenitor cells of the Drosophila larval brain [67] and is implicated in the control of NB proliferation. Bantam deletion mutants exhibit a smaller CNS and a decrease in both type I (producing ganglion mother cells) and type II (producing intermediate neural progenitors) NBs in the larval central brain. These phenotypes are associated with reduced expression of brain tumor (brat) and prospero (pros) genes, which are targeted by bantam.
miR-124 is expressed in proliferating neuronal progenitors and substantially contributes to the development of the CNS by targeting anachronism (ana), which encodes a secreted inhibitor of NB proliferation [73]. Studies using targeted miR-124 knockout mutants have demonstrated that miR-124 is crucial for neuronal progenitor cell proliferation.

4.2.2. Let-7 and miR-iab8 in the Mushroom Body (MB)

The MB is a central tissue for olfactory learning and memory, comprising four neuronal cell subtypes (γ, α′/β′, pioneer α/β, and α/β) that are generated in a specific order during Drosophila development (Figure 3) [90,91].
Several miRNAs are involved in the formation of MBs. Let-7, an ecdysone-induced miRNA, plays an important role in regulating the timing of neuronal development in the MB [69]. By targeting Chronologically inappropriate morphogenesis (chinmo), which encodes a putative BTB-zinc finger transcription factor, let-7 controls the developmental timing of neurons in the MB (Figure 3). The loss of let-7 leads to a delay in the transition of MB subtypes (γ → α′/β′ → pioneer α/β → α/β) by inhibiting chinmo, which drives the sequential generation of MB neurons.
In addition, let-7 regulates the timing of the transition from α′/β′ to α/β neuronal identities in the mushroom body by targeting another transcription factor, namely Abrupt (Ab) (Figure 3) [70]. The let-7-Ab regulatory axis influences the expression of cell adhesion molecule Fasciclin 2 (Fas2) in developing neurons. Consequently, the absence of let-7 results in learning defects due to the abnormal morphology of the MB.
Another crucial miRNA, miR-iab8, is involved in the formation of MB neurons [71]. Depletion of miR-iab8 using an miRNA sponge (SP) in the CNS and MB leads to reduced intermediate-term memory. Additionally, miR-iab8-SP-mediated inhibition causes a decrease in the number and distribution of α/β MB neurons [71]. Researchers have identified CG12229, which encodes pyruvate kinase and Ceramide phosphoethanolamine synthase (Cpes), as a potential target associated with these defects (Figure 3). Knockdown of these genes resulted in improved memory performance, contrary to the results observed with the depletion of miR-iab8 [71].

4.2.3. miR-34, miR-124, and miR-276a/b in Synaptogenesis and Dendritic Formation

miR-34 plays a crucial role in synaptogenesis in Drosophila [75]. Using RNAi, miR-34 was initially identified as an miRNA that promotes neuromuscular junction (NMJ) growth. In miR-34 mutants, defects in NMJ synapse formation have been observed, including a reduction in the expansion of motor axon terminal arbors and a decrease in the number of presynaptic boutons. Notably, miR-34 is involved in NMJ formation via distinct mechanisms in presynaptic and postsynaptic neurons [75]. In the presynaptic compartment, miR-34 inhibits junctional adhesion receptor Neurexin IV (Nrx-IV), thereby affecting active zone formation. In contrast, in the postsynaptic compartment, miR-34 suppresses the expression of membrane cytoskeletal effector protein Hu li tai shao (Hts), thereby controlling the initiation of bouton formation [75].
Furthermore, miR-124 is expressed in the CNS of Drosophila, particularly in proliferating neuronal progenitors and differentiating postmitotic neurons [73,74]. Studies have confirmed its biological significance in CNS development. Deletion of miR-124 leads to increased dendritic arborization, impaired larval locomotion, and abnormal synaptic transmission at NMJs [74]. miR-124 coordinately suppresses five positive components (saxophone [sax], thickveins [tkv], wishful thinking [wit], Mothers against dpp [Mad], and Medea [Med]) of the retrograde BMP signaling pathway in neurons.
miR-276 is associated with conserved RNA-binding protein fragile X mental retardation protein (FMRP), which is involved in dendritic arbor morphogenesis [61]. The activity of miR-276a/b is linked to the dendritic field coverage of Drosophila larval class IV da (C4da) sensory neurons by suppressing the target gene, nejire (nej). Nej functions as a transcriptional co-activator, regulating the expression of genes related to cytoskeletal dynamics, which are essential for dendritic formation. The miR-276–nej interaction is crucial for proper dendritic branching in neurons that receive signals from other neurons.

4.3. miRNAs in Wing Development

Drosophila wing development is regulated by multiple signaling pathways, such as the Hedgehog (Hh), Notch, and Wingless (Wg) pathways. Through these signaling pathways, cell proliferation, boundary formation, patterning, and morphogenesis in wing discs are regulated. Here, we discuss the regulatory roles of specific miRNAs in the signaling pathways associated with wing development.

4.3.1. miR-960 and miR-5 in the Hh Signaling Pathway of Wing Development

Distinct regulation occurs in the anterior and posterior compartments of the wing disc during wing imaginal disc development. Notably, the expression of Hh is restricted to the posterior compartment and diffuses to influence the adjacent anterior cells [92,93]. In the absence of the Hh ligand, Patched (Ptc) inhibits Smoothened (Smo), which results in the suppression of the kinase activity of the Hh complex (PKA, CK1, and GSK3) (Figure 4A) [94,95]. This suppression leads to the phosphorylation of the supernumerary limbs (Slimb), which facilitates the generation of the truncated repressor form of Cubitus interruptus (Ci) via proteasomal proteolysis. The repressor form of Ci (CiR) inhibits the expression of Hh target genes in the nucleus. In contrast, when the Hh ligand binds to Ptc, the Ptc-mediated inhibition of Smo is relieved. [94,95]. Subsequent phosphorylation by PKA and CKI leads to the formation of the Costal-2 (Cos2)-Fused (Fu) complex, leading to inhibition of the Suppressor of Fused (Sufu) complex, which suppresses Ci activation [94,95]. Consequently, the full-length active form of Ci activates Hh-dependent genes in the nucleus.
One group studied the regulation of Hh signaling by miR-5 in Drosophila wings [77]. miR-5 was identified as a negative regulator of the Hh signaling pathway by suppressing smo. Overexpression of miR-5 in the wing pouch leads to a reduced intervein region between longitudinal veins 3 and 4 (L3 and L4), which is associated with Hh signaling. Furthermore, miR-5 suppresses the expression of Hh signaling target genes such as engrailed (en), ptc, ci, and decapentaplegic (dpp). This suppression was achieved by direct targeting of smo (Figure 4A) in [77]. In addition, miR-5 appears to inhibit the Wg signaling pathway by regulating other genes and is not associated with the Notch or Dpp signaling pathways, as determined by the unchanged expression levels of Cut (ct) and Spalt major (salm), respectively [77].
Another study revealed that miR-960 suppresses Hh signaling by directly inhibiting Smo, Cos2, and Fu (Figure 4A) [76]. When the miR-960 cluster (miR-960C), comprising miR-959, miR-960, miR-961, and miR-962, is overexpressed in the wing pouch, the L3-L4 intervein region is significantly reduced. Moreover, the overexpression of miR-960C in the dorsal compartment of the wing pouch results in a marked decrease in the expression of Ptc, Col, and Ci [76].

4.3.2. miR-7 and miR-252 in the Notch Signaling Pathway of Wing Development

As another well-known crucial signaling pathway, the Notch signaling pathway is primarily involved in cell proliferation and differentiation throughout Drosophila development, particularly in the formation of the dorsal/ventral boundaries and wing-margin patterning within the wing imaginal disc [96]. In the canonical Notch signaling pathway, the interaction of the Notch receptor with membrane-bound ligands, such as Delta (Dl) and Serrate (Ser), between neighboring cells triggers the activation of Notch signaling (Figure 4B) [97,98]. This leads to two proteolytic cleavages, resulting in the release of the Notch intracellular domain (NICD). The NICD then translocates to the nucleus to activate the expression of target genes, including wg and ct [97,98].
miR-7 is expressed in wing imaginal discs [99]. Depletion of miR-7 results in reduced wing size, whereas overexpression in the wing pouch induces wing-margin notching, which is indicative of diminished Notch signaling. Consistent with this finding, the expression of ct is increased in miR-7-overexpressing wing discs. This effect may be related to the regulation of Enhancer of split complex (E(spl)-C) genes by miR-7, as determined in previous studies (Figure 4B) [78,79].
Another miRNA associated with the Notch signaling pathway, miR-252-5p, regulates Notch signaling by targeting Rab6, a member of the Rab family of small GTPases (Figure 4B) [59]. Overexpression of miR-252 in the posterior compartment of the wing disc leads to wing defects accompanied by notching of the wing blade and decreased expression of ct. Notably, miR-252-overexpressing wing discs exhibit inactivation of Notch signaling coupled with NICD accumulation due to the suppression of Rab6.

4.3.3. miR-31a/b and miR-8 in the Wg Signaling Pathway of Wing Development

The Wg pathway is one of the highly conserved signaling pathways, and the function of Wg signaling in the wing imaginal discs of Drosophila has been well elucidated [100]. In the wing discs, Wg is mainly expressed at the dorsal/ventral boundary [100]. Initially, Wg is synthesized within the Golgi apparatus and sorted into intracellular vesicles along with Wntless (Wls), a protein responsible for the secretion of Wg (Figure 4C). Subsequently, these Wg-Wls complexes are released into the extracellular space via exocytosis [101,102]. Upon release, the Wg ligand binds to the Frizzled (Fz) receptor, leading to the activation of Dishevelled (Dsh) in target cells. This inactivates the destruction complex, which comprises Adenomatous polyposis coli (APC), Axin (Axn), and Shaggy (Sgg). As a result, Armadillo (Arm) translocates into the nucleus and induces the expression of the Wg target genes, along with dTCF [103].
A conserved miRNA, miR-31, is implicated in the Wg signaling pathway by regulating transmembrane protein-encoding wls (Figure 4C), similar to its regulation in human cells [81,104]. Overexpression of both miR-31a and miR-31b in wing discs results in a significant reduction in the size of wing discs. Thus, miR-31 controls wing growth through the Wg signaling pathway.
In addition, miR-8 inhibits Wg signaling by targeting wls in Drosophila wings (Figure 4C) [63]. Additionally, miR-8 negatively regulates CG32767 [63], which encodes a zinc-finger protein identified as a positive regulator of Wg signaling [105,106]. Upon miR-8 overexpression along the anterior–posterior boundary of the wing pouch, the expression levels of Wg, Distal-less (Dll), and Fz3 are substantially reduced [63].

4.4. miRNAs in Eye Development

Drosophila compound eyes consist of approximately 800 ommatidia [107]. Each ommatidium contains eight photoreceptors (R1–8), four cone cells, two primary pigment cells, six secondary pigment cells, three tertiary pigment cells, and three bristle complexes. Among the photoreceptors, the R1–6 cells are located in the outer regions, whereas the R7 and R8 cells are centrally located. The R7 cells are positioned above the R8 cells.
Eye development, including distinct cell fates and structural formation, is coordinated by multiple signaling pathways [107]. Following R8 photoreceptor specification mediated by Notch signaling, epidermal growth factor receptor (EGFR) and receptor tyrosine kinase (RTK) signaling facilitate the recruitment of R2/5, R3/4, R1/6, and R7 photoreceptors to each ommatidial cluster (Figure 5) [82,108]. Sevenless (Sev) receptor-mediated RTK signaling specifies the final photoreceptor, R7.
miR-7 is involved in photoreceptor differentiation in Drosophila eyes through the EGFR signaling pathway [80]. In situ hybridization confirmed that miR-7 is expressed and active in the development of photoreceptors. In the ommatidia of miR-7 deletion mutants, only ectopic R7 photoreceptors—and not ectopic cone cells—were observed, indicating that miR-7 is specifically associated with photoreceptor differentiation. Additional analysis revealed that miR-7 negatively regulates the E26 transformation-specific (ETS) domain transcription factor Yan (also known as anterior open [aop]), consequently stimulating photoreceptor differentiation (Figure 5) [80]. Furthermore, the derepression of Yan, mediated by the activation of EGFR signaling, induces the expression of miR-7, in addition to Yan regulation by miR-7 [80]. This reciprocal regulation of miR-7 and Yan controls eye development in Drosophila.
As for other eye development-associated miRNAs, miR-279 and miR-996 are essential for normal eye development [82]. MiR-279 and miR-996 are co-expressed and have identical seed sequences [109]. Deletion of miR-279 and miR-996 results in eye roughening [82]. When adult eyes are sectioned, seven of the eight photoreceptor rhabdomeres can be observed in the case of normal eyes, including six outer photoreceptors (R1–6) and one inner photoreceptor (either R7 or R8, depending on the position of the section). However, the adult eyes of miR-279 and miR-996 deletion mutants abnormally exhibit multiple ectopic R7 cells. Furthermore, in miR-279 and miR-996 mutants, the number of Arm + photoreceptor cells increases, while the number of cone cells decreases. These defects are associated with components of the RTK/EGFR signaling pathway, such as rhomboid (rho), roughoid (ru), and bride of sevenless (boss), which are regulated by miR-279 and miR-996 (Figure 5).

5. Discussion and Future Research Directions

In the last 20 years, numerous studies on Drosophila miRNAs have revealed a relationship between over 150 miRNA target genes. However, compared with the numerous potential target genes predicted for each miRNA by TargetScanFly, this number remains relatively small. Moreover, the biological roles of a substantial proportion of the 469 mature miRNAs in Drosophila remain unexplored. Thus, further investigation of miRNAs is essential for understanding gene regulation across diverse developmental processes.
To comprehensively study the biological roles of miRNAs, it is critical to identify the target genes regulated by individual miRNAs. With the development and improvement of high-throughput sequencing techniques and computational biology tools, clearer information regarding the interactions between miRNAs and their target mRNAs can be obtained. CLIP-seq techniques, including high-throughput sequencing CLIP (HITS-CLIP), photoactivatable ribonucleoside-enhanced CLIP (PAR-CLIP), individual-nucleotide resolution CLIP (iCLIP), and enhanced CLIP (eCLIP), allow for the capture of RNAs that interact with specific RNA-binding proteins (Table 2) [110,111,112,113]. By applying this method to Ago proteins involved in miRNA pathways, Ago-binding miRNAs and Ago-binding mRNA regions can be identified. Then, using computational tools, substantial interactions between individual miRNAs and their target regions can be deduced. In Drosophila, several groups have identified these interactions using the Ago1-CLIP-seq method [50,51,114], facilitating an understanding of the regulatory network mediated by miRNAs.
However, CLIP-seq is not a technique to directly capture miRNA–target mRNA interactions. To address this limitation, sequencing techniques, such as crosslinking, ligation, and sequencing of hybrids (CLASH) and covalent ligation of endogenous Argonaute-bound RNAs-CLIP (CLEAR-CLIP), have been developed and employed to study miRNA–target mRNA interactions in human cells (Table 2) [115,116]. Recently, RNA in situ conformation sequencing (RIC-seq), a method to capture global RNA-RNA interactions, has also been developed, allowing us to obtain information on miRNA–target mRNA interactions (Table 2) [117]. Therefore, to study the regulatory roles of individual miRNAs in Drosophila development, cutting-edge sequencing technologies are necessary. Due to the plasticity of the interactions between miRNAs and target mRNA, these techniques should be performed under various conditions, such as at different developmental stages and in different tissues. Through these approaches, the complex networks of miRNA–mRNA interactions will be revealed in various developmental processes.
In addition, based on the vast interaction data obtained from sequencing techniques at each developmental time point and in specific tissues, comprehensive regulatory networks between multiple central miRNAs and their target genes should be simultaneously analyzed to understand complex developmental processes. However, to date, almost all studies have focused on only one or two miRNA target genes in a single context. In reality, one miRNA can regulate the expression of many genes by binding to specific regions within the 3′-UTR of multiple targets in an imperfect-match manner [118]. Conversely, multiple miRNAs can simultaneously modulate one target gene. Therefore, we should analyze the regulatory consequences mediated by miRNAs with different expression strengths and directions depending on the spatial and temporal conditions of development.
Furthermore, compared with the expected miRNA–target gene interactions in Drosophila development, only a small portion of miRNA–target gene interactions have been experimentally validated. Numerous networks remain unknown under various developmental conditions. Therefore, in addition to sequencing methods, efforts are needed to uncover the individual relationships between miRNAs and target genes using various traditional approaches for miRNA studies, such as reporter assays. Through these efforts, it is expected that, in the near future, the puzzle of the regulatory mechanisms of miRNAs in developmental processes will be solved, leading to a broader understanding of the developmental processes of Drosophila.

Author Contributions

Conceptualization: D.J., C.J.K. and D.-H.L.; investigation: D.J., C.J.K. and B.H.S.; writing—original draft preparation: D.J., C.J.K., B.H.S. and D.-H.L.; writing—review and editing: D.-H.L.; visualization: C.J.K., B.H.S. and D.-H.L.; supervision: D.-H.L.; funding acquisition: D.-H.L. All authors have read and agreed to the published version of the manuscript.

Funding

This work was supported by the Soongsil University Research Fund (New Professor Support Research), 2021.

Data Availability Statement

Data are contained within the article.

Conflicts of Interest

The authors declare no conflicts of interest.

References

  1. He, L.; Hannon, G.J. MicroRNAs: Small RNAs with a big role in gene regulation. Nat. Rev. Genet. 2004, 5, 522–531. [Google Scholar] [CrossRef]
  2. Chyb, S.; Gompel, N. Atlas of Drosophila Morphology: Wild-Type and Classical Mutants; Academic Press: London, UK, 2013. [Google Scholar]
  3. Wightman, B.; Ha, I.; Ruvkun, G. Posttranscriptional regulation of the heterochronic gene lin-14 by lin-4 mediates temporal pattern formation in C. elegans. Cell 1993, 75, 855–862. [Google Scholar] [CrossRef]
  4. Lee, R.C.; Feinbaum, R.L.; Ambros, V. The C. elegans heterochronic gene lin-4 encodes small RNAs with antisense complementarity to lin-14. Cell 1993, 75, 843–854. [Google Scholar] [CrossRef]
  5. Lagos-Quintana, M.; Rauhut, R.; Lendeckel, W.; Tuschl, T. Identification of novel genes coding for small expressed RNAs. Science 2001, 294, 853–858. [Google Scholar] [CrossRef]
  6. Aravin, A.A.; Lagos-Quintana, M.; Yalcin, A.; Zavolan, M.; Marks, D.; Snyder, B.; Gaasterland, T.; Meyer, J.; Tuschl, T. The small RNA profile during Drosophila melanogaster development. Dev. Cell 2003, 5, 337–350. [Google Scholar] [CrossRef]
  7. Ruby, J.G.; Stark, A.; Johnston, W.K.; Kellis, M.; Bartel, D.P.; Lai, E.C. Evolution, biogenesis, expression, and target predictions of a substantially expanded set of Drosophila microRNAs. Genome Res. 2007, 17, 1850–1864. [Google Scholar] [CrossRef]
  8. Stark, A.; Kheradpour, P.; Parts, L.; Brennecke, J.; Hodges, E.; Hannon, G.J.; Kellis, M. Systematic discovery and characterization of fly microRNAs using 12 Drosophila genomes. Genome Res. 2007, 17, 1865–1879. [Google Scholar] [CrossRef]
  9. Griffiths-Jones, S.; Grocock, R.J.; van Dongen, S.; Bateman, A.; Enright, A.J. miRBase: microRNA sequences, targets and gene nomenclature. Nucleic Acids Res. 2006, 34, D140–D144. [Google Scholar] [CrossRef]
  10. Chawla, G.; Sokol, N.S. MicroRNAs in Drosophila development. Int. Rev. Cell Mol. Biol. 2011, 286, 1–65. [Google Scholar] [CrossRef]
  11. Quesnelle, D.C.; Bendena, W.G.; Chin-Sang, I.D. A Compilation of the Diverse miRNA Functions in Caenorhabditis elegans and Drosophila melanogaster Development. Int. J. Mol. Sci. 2023, 24, 6963. [Google Scholar] [CrossRef]
  12. Lee, Y.; Kim, M.; Han, J.; Yeom, K.H.; Lee, S.; Baek, S.H.; Kim, V.N. MicroRNA genes are transcribed by RNA polymerase II. EMBO J. 2004, 23, 4051–4060. [Google Scholar] [CrossRef]
  13. Cai, X.; Hagedorn, C.H.; Cullen, B.R. Human microRNAs are processed from capped, polyadenylated transcripts that can also function as mRNAs. RNA 2004, 10, 1957–1966. [Google Scholar] [CrossRef]
  14. Borchert, G.M.; Lanier, W.; Davidson, B.L. RNA polymerase III transcribes human microRNAs. Nat. Struct. Mol. Biol. 2006, 13, 1097–1101. [Google Scholar] [CrossRef]
  15. Lee, Y.; Jeon, K.; Lee, J.T.; Kim, S.; Kim, V.N. MicroRNA maturation: Stepwise processing and subcellular localization. EMBO J. 2002, 21, 4663–4670. [Google Scholar] [CrossRef]
  16. Han, J.; Lee, Y.; Yeom, K.H.; Kim, Y.K.; Jin, H.; Kim, V.N. The Drosha-DGCR8 complex in primary microRNA processing. Genes Dev. 2004, 18, 3016–3027. [Google Scholar] [CrossRef]
  17. Gregory, R.I.; Yan, K.P.; Amuthan, G.; Chendrimada, T.; Doratotaj, B.; Cooch, N.; Shiekhattar, R. The Microprocessor complex mediates the genesis of microRNAs. Nature 2004, 432, 235–240. [Google Scholar] [CrossRef]
  18. Denli, A.M.; Tops, B.B.; Plasterk, R.H.; Ketting, R.F.; Hannon, G.J. Processing of primary microRNAs by the Microprocessor complex. Nature 2004, 432, 231–235. [Google Scholar] [CrossRef]
  19. Morlando, M.; Ballarino, M.; Gromak, N.; Pagano, F.; Bozzoni, I.; Proudfoot, N.J. Primary microRNA transcripts are processed co-transcriptionally. Nat. Struct. Mol. Biol. 2008, 15, 902–909. [Google Scholar] [CrossRef]
  20. Okamura, K.; Hagen, J.W.; Duan, H.; Tyler, D.M.; Lai, E.C. The mirtron pathway generates microRNA-class regulatory RNAs in Drosophila. Cell 2007, 130, 89–100. [Google Scholar] [CrossRef]
  21. Ruby, J.G.; Jan, C.H.; Bartel, D.P. Intronic microRNA precursors that bypass Drosha processing. Nature 2007, 448, 83–86. [Google Scholar] [CrossRef]
  22. Shibata, S.; Sasaki, M.; Miki, T.; Shimamoto, A.; Furuichi, Y.; Katahira, J.; Yoneda, Y. Exportin-5 orthologues are functionally divergent among species. Nucleic Acids Res. 2006, 34, 4711–4721. [Google Scholar] [CrossRef]
  23. Yi, R.; Qin, Y.; Macara, I.G.; Cullen, B.R. Exportin-5 mediates the nuclear export of pre-microRNAs and short hairpin RNAs. Genes Dev. 2003, 17, 3011–3016. [Google Scholar] [CrossRef]
  24. Lund, E.; Guttinger, S.; Calado, A.; Dahlberg, J.E.; Kutay, U. Nuclear export of microRNA precursors. Science 2004, 303, 95–98. [Google Scholar] [CrossRef]
  25. Hutvagner, G.; McLachlan, J.; Pasquinelli, A.E.; Balint, E.; Tuschl, T.; Zamore, P.D. A cellular function for the RNA-interference enzyme Dicer in the maturation of the let-7 small temporal RNA. Science 2001, 293, 834–838. [Google Scholar] [CrossRef]
  26. Knight, S.W.; Bass, B.L. A role for the RNase III enzyme DCR-1 in RNA interference and germ line development in Caenorhabditis elegans. Science 2001, 293, 2269–2271. [Google Scholar] [CrossRef]
  27. Grishok, A.; Pasquinelli, A.E.; Conte, D.; Li, N.; Parrish, S.; Ha, I.; Baillie, D.L.; Fire, A.; Ruvkun, G.; Mello, C.C. Genes and mechanisms related to RNA interference regulate expression of the small temporal RNAs that control C. elegans developmental timing. Cell 2001, 106, 23–34. [Google Scholar] [CrossRef]
  28. Lee, Y.S.; Nakahara, K.; Pham, J.W.; Kim, K.; He, Z.; Sontheimer, E.J.; Carthew, R.W. Distinct roles for Drosophila Dicer-1 and Dicer-2 in the siRNA/miRNA silencing pathways. Cell 2004, 117, 69–81. [Google Scholar] [CrossRef]
  29. Macrae, I.J.; Zhou, K.; Li, F.; Repic, A.; Brooks, A.N.; Cande, W.Z.; Adams, P.D.; Doudna, J.A. Structural basis for double-stranded RNA processing by Dicer. Science 2006, 311, 195–198. [Google Scholar] [CrossRef]
  30. Zhang, H.; Kolb, F.A.; Jaskiewicz, L.; Westhof, E.; Filipowicz, W. Single processing center models for human Dicer and bacterial RNase III. Cell 2004, 118, 57–68. [Google Scholar] [CrossRef]
  31. Kawamata, T.; Tomari, Y. Making RISC. Trends Biochem. Sci. 2010, 35, 368–376. [Google Scholar] [CrossRef]
  32. Forstemann, K.; Horwich, M.D.; Wee, L.; Tomari, Y.; Zamore, P.D. Drosophila microRNAs are sorted into functionally distinct argonaute complexes after production by dicer-1. Cell 2007, 130, 287–297. [Google Scholar] [CrossRef]
  33. Okamura, K.; Ishizuka, A.; Siomi, H.; Siomi, M.C. Distinct roles for Argonaute proteins in small RNA-directed RNA cleavage pathways. Genes Dev. 2004, 18, 1655–1666. [Google Scholar] [CrossRef] [PubMed]
  34. Schwarz, D.S.; Hutvagner, G.; Du, T.; Xu, Z.; Aronin, N.; Zamore, P.D. Asymmetry in the assembly of the RNAi enzyme complex. Cell 2003, 115, 199–208. [Google Scholar] [CrossRef] [PubMed]
  35. Khvorova, A.; Reynolds, A.; Jayasena, S.D. Functional siRNAs and miRNAs exhibit strand bias. Cell 2003, 115, 209–216. [Google Scholar] [CrossRef] [PubMed]
  36. Hammond, S.M. Dicing and slicing: The core machinery of the RNA interference pathway. FEBS Lett. 2005, 579, 5822–5829. [Google Scholar] [CrossRef] [PubMed]
  37. Zhang, X.; Li, S.; Liu, S. Juvenile Hormone Studies in Drosophila melanogaster. Front. Physiol. 2021, 12, 785320. [Google Scholar] [CrossRef]
  38. Jindra, M.; Uhlirova, M.; Charles, J.P.; Smykal, V.; Hill, R.J. Genetic Evidence for Function of the bHLH-PAS Protein Gce/Met As a Juvenile Hormone Receptor. PLoS Genet. 2015, 11, e1005394. [Google Scholar] [CrossRef] [PubMed]
  39. Li, M.; Mead, E.A.; Zhu, J. Heterodimer of two bHLH-PAS proteins mediates juvenile hormone-induced gene expression. Proc. Natl. Acad. Sci. USA 2011, 108, 638–643. [Google Scholar] [CrossRef]
  40. He, Q.; Wen, D.; Jia, Q.; Cui, C.; Wang, J.; Palli, S.R.; Li, S. Heat shock protein 83 (Hsp83) facilitates methoprene-tolerant (Met) nuclear import to modulate juvenile hormone signaling. J. Biol. Chem. 2014, 289, 27874–27885. [Google Scholar] [CrossRef]
  41. He, Q.; Zhang, Y.; Zhang, X.; Xu, D.; Dong, W.; Li, S.; Wu, R. Nucleoporin Nup358 facilitates nuclear import of Methoprene-tolerant (Met) in an importin β- and Hsp83-dependent manner. Insect Biochem. Mol. Biol. 2017, 81, 10–18. [Google Scholar] [CrossRef]
  42. Yamanaka, N.; Rewitz, K.F.; O’Connor, M.B. Ecdysone control of developmental transitions: Lessons from Drosophila research. Annu. Rev. Entomol. 2013, 58, 497–516. [Google Scholar] [CrossRef] [PubMed]
  43. Truman, J.W.; Riddiford, L.M. Endocrine insights into the evolution of metamorphosis in insects. Annu. Rev. Entomol. 2002, 47, 467–500. [Google Scholar] [CrossRef] [PubMed]
  44. Yao, T.P.; Forman, B.M.; Jiang, Z.; Cherbas, L.; Chen, J.D.; McKeown, M.; Cherbas, P.; Evans, R.M. Functional ecdysone receptor is the product of EcR and Ultraspiracle genes. Nature 1993, 366, 476–479. [Google Scholar] [CrossRef] [PubMed]
  45. Yao, T.P.; Segraves, W.A.; Oro, A.E.; McKeown, M.; Evans, R.M. Drosophila ultraspiracle modulates ecdysone receptor function via heterodimer formation. Cell 1992, 71, 63–72. [Google Scholar] [CrossRef] [PubMed]
  46. DiBello, P.R.; Withers, D.A.; Bayer, C.A.; Fristrom, J.W.; Guild, G.M. The Drosophila Broad-Complex encodes a family of related proteins containing zinc fingers. Genetics 1991, 129, 385–397. [Google Scholar] [CrossRef] [PubMed]
  47. Segraves, W.A.; Hogness, D.S. The E75 ecdysone-inducible gene responsible for the 75B early puff in Drosophila encodes two new members of the steroid receptor superfamily. Genes Dev. 1990, 4, 204–219. [Google Scholar] [CrossRef] [PubMed]
  48. Burtis, K.C.; Thummel, C.S.; Jones, C.W.; Karim, F.D.; Hogness, D.S. The Drosophila 74EF early puff contains E74, a complex ecdysone-inducible gene that encodes two ets-related proteins. Cell 1990, 61, 85–99. [Google Scholar] [CrossRef] [PubMed]
  49. Riddiford, L.M.; Cherbas, P.; Truman, J.W. Ecdysone receptors and their biological actions. Vitam. Horm. 2000, 60, 1–73. [Google Scholar] [CrossRef]
  50. Lim, D.H.; Lee, S.; Han, J.Y.; Choi, M.S.; Hong, J.S.; Seong, Y.; Kwon, Y.S.; Lee, Y.S. Ecdysone-responsive microRNA-252-5p controls the cell cycle by targeting Abi in Drosophila. FASEB J. 2018, 32, 4519–4533. [Google Scholar] [CrossRef]
  51. Lim, D.H.; Lee, S.; Choi, M.S.; Han, J.Y.; Seong, Y.; Na, D.; Kwon, Y.S.; Lee, Y.S. The conserved microRNA miR-8-3p coordinates the expression of V-ATPase subunits to regulate ecdysone biosynthesis for Drosophila metamorphosis. FASEB J. 2020, 34, 6449–6465. [Google Scholar] [CrossRef]
  52. Sempere, L.F.; Sokol, N.S.; Dubrovsky, E.B.; Berger, E.M.; Ambros, V. Temporal regulation of microRNA expression in Drosophila melanogaster mediated by hormonal signals and broad-Complex gene activity. Dev. Biol. 2003, 259, 9–18. [Google Scholar] [CrossRef]
  53. Sokol, N.S.; Xu, P.; Jan, Y.N.; Ambros, V. Drosophila let-7 microRNA is required for remodeling of the neuromusculature during metamorphosis. Genes Dev. 2008, 22, 1591–1596. [Google Scholar] [CrossRef]
  54. Jin, X.; Wu, X.; Zhou, L.; He, T.; Yin, Q.; Liu, S. 20-Hydroxyecdysone-responsive microRNAs of insects. RNA Biol. 2020, 17, 1454–1471. [Google Scholar] [CrossRef]
  55. He, Q.; Zhang, Y.; Dong, W. MicroRNA miR-927 targets the juvenile hormone primary response gene Kruppel homolog1 to control Drosophila developmental growth. Insect Mol. Biol. 2020, 29, 545–554. [Google Scholar] [CrossRef]
  56. Garbuzov, A.; Tatar, M. Hormonal regulation of Drosophila microRNA let-7 and miR-125 that target innate immunity. Fly 2010, 4, 306–311. [Google Scholar] [CrossRef]
  57. Chan, K.K.; Chan, T.F.; Bendena, W.; Hui, J.H.L. Noncoding RNA Regulation of Hormonal and Metabolic Systems in the Fruit Fly Drosophila. Metabolites 2023, 13, 152. [Google Scholar] [CrossRef]
  58. Lim, D.H.; Lee, S.; Han, J.Y.; Choi, M.S.; Hong, J.S.; Lee, Y.S. MicroRNA miR-252 targets mbt to control the developmental growth of Drosophila. Insect Mol. Biol. 2019, 28, 444–454. [Google Scholar] [CrossRef]
  59. Lim, D.H.; Choi, M.S.; Jeon, J.W.; Lee, Y.S. MicroRNA miR-252-5p regulates the Notch signaling pathway by targeting Rab6 in Drosophila wing development. Insect Sci. 2023, 30, 1431–1444. [Google Scholar] [CrossRef]
  60. Lee, S.; Kim, N.; Jang, D.; Kim, H.K.; Kim, J.; Jeon, J.W.; Lim, D.H. Ecdysone-induced microRNA miR-276a-3p controls developmental growth by targeting the insulin-like receptor in Drosophila. Insect Mol. Biol. 2023, 32, 703–715. [Google Scholar] [CrossRef]
  61. Li, H.; Gavis, E.R. Drosophila FMRP controls miR-276-mediated regulation of nejire mRNA for space-filling dendrite development. G3 2022, 12, jkac239. [Google Scholar] [CrossRef]
  62. Hyun, S.; Lee, J.H.; Jin, H.; Nam, J.; Namkoong, B.; Lee, G.; Chung, J.; Kim, V.N. Conserved MicroRNA miR-8/miR-200 and its target USH/FOG2 control growth by regulating PI3K. Cell 2009, 139, 1096–1108. [Google Scholar] [CrossRef] [PubMed]
  63. Kennell, J.A.; Gerin, I.; MacDougald, O.A.; Cadigan, K.M. The microRNA miR-8 is a conserved negative regulator of Wnt signaling. Proc. Natl. Acad. Sci. USA 2008, 105, 15417–15422. [Google Scholar] [CrossRef] [PubMed]
  64. Varghese, J.; Lim, S.F.; Cohen, S.M. Drosophila miR-14 regulates insulin production and metabolism through its target, sugarbabe. Genes Dev. 2010, 24, 2748–2753. [Google Scholar] [CrossRef] [PubMed]
  65. Xu, P.; Vernooy, S.Y.; Guo, M.; Hay, B.A. The Drosophila microRNA Mir-14 suppresses cell death and is required for normal fat metabolism. Curr. Biol. 2003, 13, 790–795. [Google Scholar] [CrossRef] [PubMed]
  66. Brennecke, J.; Hipfner, D.R.; Stark, A.; Russell, R.B.; Cohen, S.M. bantam encodes a developmentally regulated microRNA that controls cell proliferation and regulates the proapoptotic gene hid in Drosophila. Cell 2003, 113, 25–36. [Google Scholar] [CrossRef]
  67. Weng, R.; Cohen, S.M. Control of Drosophila Type I and Type II central brain neuroblast proliferation by bantam microRNA. Development 2015, 142, 3713–3720. [Google Scholar] [CrossRef]
  68. Ge, W.; Chen, Y.W.; Weng, R.; Lim, S.F.; Buescher, M.; Zhang, R.; Cohen, S.M. Overlapping functions of microRNAs in control of apoptosis during Drosophila embryogenesis. Cell Death Differ. 2012, 19, 839–846. [Google Scholar] [CrossRef] [PubMed]
  69. Wu, Y.C.; Chen, C.H.; Mercer, A.; Sokol, N.S. Let-7-complex microRNAs regulate the temporal identity of Drosophila mushroom body neurons via chinmo. Dev. Cell 2012, 23, 202–209. [Google Scholar] [CrossRef] [PubMed]
  70. Kucherenko, M.M.; Barth, J.; Fiala, A.; Shcherbata, H.R. Steroid-induced microRNA let-7 acts as a spatio-temporal code for neuronal cell fate in the developing Drosophila brain. EMBO J. 2012, 31, 4511–4523. [Google Scholar] [CrossRef]
  71. Busto, G.U.; Guven-Ozkan, T.; Chakraborty, M.; Davis, R.L. Developmental inhibition of miR-iab8-3p disrupts mushroom body neuron structure and adult learning ability. Dev. Biol. 2016, 419, 237–249. [Google Scholar] [CrossRef]
  72. Yuva-Aydemir, Y.; Xu, X.L.; Aydemir, O.; Gascon, E.; Sayin, S.; Zhou, W.; Hong, Y.; Gao, F.B. Downregulation of the Host Gene jigr1 by miR-92 Is Essential for Neuroblast Self-Renewal in Drosophila. PLoS Genet. 2015, 11, e1005264. [Google Scholar] [CrossRef]
  73. Weng, R.; Cohen, S.M. Drosophila miR-124 regulates neuroblast proliferation through its target anachronism. Development 2012, 139, 1427–1434. [Google Scholar] [CrossRef] [PubMed]
  74. Sun, K.; Westholm, J.O.; Tsurudome, K.; Hagen, J.W.; Lu, Y.; Kohwi, M.; Betel, D.; Gao, F.B.; Haghighi, A.P.; Doe, C.Q.; et al. Neurophysiological defects and neuronal gene deregulation in Drosophila mir-124 mutants. PLoS Genet. 2012, 8, e1002515. [Google Scholar] [CrossRef]
  75. McNeill, E.M.; Warinner, C.; Alkins, S.; Taylor, A.; Heggeness, H.; DeLuca, T.F.; Fulga, T.A.; Wall, D.P.; Griffith, L.C.; Van Vactor, D. The conserved microRNA miR-34 regulates synaptogenesis via coordination of distinct mechanisms in presynaptic and postsynaptic cells. Nat. Commun. 2020, 11, 1092. [Google Scholar] [CrossRef]
  76. Gao, L.; Hou, X.; Wu, L.; Zhang, F.; Zhang, Q.; Ye, X.; Yang, Y.; Lin, X. Drosophila miR-960 negatively regulates Hedgehog signaling by suppressing Smoothened, Costal-2 and Fused. Cell. Signal. 2013, 25, 1301–1309. [Google Scholar] [CrossRef]
  77. Wu, L.F.; Gao, L.; Hou, X.M.; Zhang, Q.H.; Li, S.; Yang, Y.F.; Lin, X.H. Drosophila miR-5 suppresses Hedgehog signaling by directly targeting Smoothened. FEBS Lett. 2012, 586, 4052–4060. [Google Scholar] [CrossRef]
  78. Stark, A.; Brennecke, J.; Russell, R.B.; Cohen, S.M. Identification of Drosophila MicroRNA targets. PLoS Biol. 2003, 1, E60. [Google Scholar] [CrossRef]
  79. Lai, E.C.; Tam, B.; Rubin, G.M. Pervasive regulation of Drosophila Notch target genes by GY-box-, Brd-box-, and K-box-class microRNAs. Genes Dev. 2005, 19, 1067–1080. [Google Scholar] [CrossRef]
  80. Li, X.; Carthew, R.W. A microRNA mediates EGF receptor signaling and promotes photoreceptor differentiation in the Drosophila eye. Cell 2005, 123, 1267–1277. [Google Scholar] [CrossRef]
  81. Jung, J.E.; Lee, J.Y.; Kim, I.R.; Park, S.M.; Kang, J.W.; Kim, Y.H.; Park, H.R.; Lee, J.H. MicroRNA-31 Regulates Expression of Wntless in Both Drosophila melanogaster and Human Oral Cancer Cells. Int. J. Mol. Sci. 2020, 21, 7232. [Google Scholar] [CrossRef] [PubMed]
  82. Duan, H.; de Navas, L.F.; Hu, F.; Sun, K.; Mavromatakis, Y.E.; Viets, K.; Zhou, C.; Kavaler, J.; Johnston, R.J.; Tomlinson, A.; et al. The mir-279/996 cluster represses receptor tyrosine kinase signaling to determine cell fates in the Drosophila eye. Development 2018, 145, dev159053. [Google Scholar] [CrossRef] [PubMed]
  83. Edgar, B.A. How flies get their size: Genetics meets physiology. Nat. Rev. Genet 2006, 7, 907–916. [Google Scholar] [CrossRef] [PubMed]
  84. Liguori, F.; Mascolo, E.; Verni, F. The Genetics of Diabetes: What We Can Learn from Drosophila. Int. J. Mol. Sci. 2021, 22, 11295. [Google Scholar] [CrossRef] [PubMed]
  85. Varghese, J.; Cohen, S.M. microRNA miR-14 acts to modulate a positive autoregulatory loop controlling steroid hormone signaling in Drosophila. Genes Dev. 2007, 21, 2277–2282. [Google Scholar] [CrossRef] [PubMed]
  86. Steller, H. Regulation of apoptosis in Drosophila. Cell Death Differ. 2008, 15, 1132–1138. [Google Scholar] [CrossRef]
  87. Denton, D.; Aung-Htut, M.T.; Kumar, S. Developmentally programmed cell death in Drosophila. Biochim. Biophys. Acta 2013, 1833, 3499–3506. [Google Scholar] [CrossRef] [PubMed]
  88. Bejarano, F.; Chang, C.H.; Sun, K.; Hagen, J.W.; Deng, W.M.; Lai, E.C. A comprehensive in vivo screen for anti-apoptotic miRNAs indicates broad capacities for oncogenic synergy. Dev. Biol. 2021, 475, 10–20. [Google Scholar] [CrossRef] [PubMed]
  89. Homem, C.C.; Knoblich, J.A. Drosophila neuroblasts: A model for stem cell biology. Development 2012, 139, 4297–4310. [Google Scholar] [CrossRef] [PubMed]
  90. Lee, T.; Lee, A.; Luo, L. Development of the Drosophila mushroom bodies: Sequential generation of three distinct types of neurons from a neuroblast. Development 1999, 126, 4065–4076. [Google Scholar] [CrossRef]
  91. Zhu, S.; Chiang, A.S.; Lee, T. Development of the Drosophila mushroom bodies: Elaboration, remodeling and spatial organization of dendrites in the calyx. Development 2003, 130, 2603–2610. [Google Scholar] [CrossRef]
  92. Tabata, T.; Kornberg, T.B. Hedgehog is a signaling protein with a key role in patterning Drosophila imaginal discs. Cell 1994, 76, 89–102. [Google Scholar] [CrossRef] [PubMed]
  93. Basler, K.; Struhl, G. Compartment boundaries and the control of Drosophila limb pattern by hedgehog protein. Nature 1994, 368, 208–214. [Google Scholar] [CrossRef]
  94. Hooper, J.E.; Scott, M.P. Communicating with Hedgehogs. Nat. Rev. Mol. Cell Biol. 2005, 6, 306–317. [Google Scholar] [CrossRef]
  95. Huangfu, D.; Anderson, K.V. Signaling from Smo to Ci/Gli: Conservation and divergence of Hedgehog pathways from Drosophila to vertebrates. Development 2006, 133, 3–14. [Google Scholar] [CrossRef]
  96. Irvine, K.D.; Vogt, T.F. Dorsal-ventral signaling in limb development. Curr. Opin. Cell Biol. 1997, 9, 867–876. [Google Scholar] [CrossRef] [PubMed]
  97. Kopan, R.; Ilagan, M.X. The canonical Notch signaling pathway: Unfolding the activation mechanism. Cell 2009, 137, 216–233. [Google Scholar] [CrossRef]
  98. Bray, S.J. Notch signalling: A simple pathway becomes complex. Nat. Rev. Mol. Cell Biol. 2006, 7, 678–689. [Google Scholar] [CrossRef] [PubMed]
  99. Aparicio, R.; Simoes Da Silva, C.J.; Busturia, A. MicroRNA miR-7 contributes to the control of Drosophila wing growth. Dev. Dyn. 2015, 244, 21–30. [Google Scholar] [CrossRef]
  100. Swarup, S.; Verheyen, E.M. Wnt/Wingless signaling in Drosophila. Cold Spring Harb. Perspect. Biol. 2012, 4, a007930. [Google Scholar] [CrossRef] [PubMed]
  101. Yu, J.; Chia, J.; Canning, C.A.; Jones, C.M.; Bard, F.A.; Virshup, D.M. WLS retrograde transport to the endoplasmic reticulum during Wnt secretion. Dev. Cell 2014, 29, 277–291. [Google Scholar] [CrossRef]
  102. Port, F.; Kuster, M.; Herr, P.; Furger, E.; Banziger, C.; Hausmann, G.; Basler, K. Wingless secretion promotes and requires retromer-dependent cycling of Wntless. Nat. Cell Biol. 2008, 10, 178–185. [Google Scholar] [CrossRef] [PubMed]
  103. Waghmare, I.; Page-McCaw, A. Wnt Signaling in Stem Cell Maintenance and Differentiation in the Drosophila Germarium. Genes 2018, 9, 127. [Google Scholar] [CrossRef]
  104. Goodman, R.M.; Thombre, S.; Firtina, Z.; Gray, D.; Betts, D.; Roebuck, J.; Spana, E.P.; Selva, E.M. Sprinter: A novel transmembrane protein required for Wg secretion and signaling. Development 2006, 133, 4901–4911. [Google Scholar] [CrossRef]
  105. DasGupta, R.; Kaykas, A.; Moon, R.T.; Perrimon, N. Functional genomic analysis of the Wnt-wingless signaling pathway. Science 2005, 308, 826–833. [Google Scholar] [CrossRef]
  106. DasGupta, R.; Nybakken, K.; Booker, M.; Mathey-Prevot, B.; Gonsalves, F.; Changkakoty, B.; Perrimon, N. A case study of the reproducibility of transcriptional reporter cell-based RNAi screens in Drosophila. Genome Biol. 2007, 8, R203. [Google Scholar] [CrossRef] [PubMed]
  107. Kumar, J.P. Building an ommatidium one cell at a time. Dev. Dyn. 2012, 241, 136–149. [Google Scholar] [CrossRef]
  108. Freeman, M. Reiterative use of the EGF receptor triggers differentiation of all cell types in the Drosophila eye. Cell 1996, 87, 651–660. [Google Scholar] [CrossRef] [PubMed]
  109. Sun, K.; Jee, D.; de Navas, L.F.; Duan, H.; Lai, E.C. Multiple In Vivo Biological Processes Are Mediated by Functionally Redundant Activities of Drosophila mir-279 and mir-996. PLoS Genet. 2015, 11, e1005245. [Google Scholar] [CrossRef]
  110. Chi, S.W.; Zang, J.B.; Mele, A.; Darnell, R.B. Argonaute HITS-CLIP decodes microRNA-mRNA interaction maps. Nature 2009, 460, 479–486. [Google Scholar] [CrossRef]
  111. Hafner, M.; Landthaler, M.; Burger, L.; Khorshid, M.; Hausser, J.; Berninger, P.; Rothballer, A.; Ascano, M., Jr.; Jungkamp, A.C.; Munschauer, M.; et al. Transcriptome-wide identification of RNA-binding protein and microRNA target sites by PAR-CLIP. Cell 2010, 141, 129–141. [Google Scholar] [CrossRef]
  112. Konig, J.; Zarnack, K.; Rot, G.; Curk, T.; Kayikci, M.; Zupan, B.; Turner, D.J.; Luscombe, N.M.; Ule, J. iCLIP reveals the function of hnRNP particles in splicing at individual nucleotide resolution. Nat. Struct. Mol. Biol. 2010, 17, 909–915. [Google Scholar] [CrossRef]
  113. Van Nostrand, E.L.; Pratt, G.A.; Shishkin, A.A.; Gelboin-Burkhart, C.; Fang, M.Y.; Sundararaman, B.; Blue, S.M.; Nguyen, T.B.; Surka, C.; Elkins, K.; et al. Robust transcriptome-wide discovery of RNA-binding protein binding sites with enhanced CLIP (eCLIP). Nat. Methods 2016, 13, 508–514. [Google Scholar] [CrossRef]
  114. Wessels, H.H.; Lebedeva, S.; Hirsekorn, A.; Wurmus, R.; Akalin, A.; Mukherjee, N.; Ohler, U. Global identification of functional microRNA-mRNA interactions in Drosophila. Nat. Commun. 2019, 10, 1626. [Google Scholar] [CrossRef]
  115. Helwak, A.; Kudla, G.; Dudnakova, T.; Tollervey, D. Mapping the human miRNA interactome by CLASH reveals frequent noncanonical binding. Cell 2013, 153, 654–665. [Google Scholar] [CrossRef]
  116. Moore, M.J.; Scheel, T.K.; Luna, J.M.; Park, C.Y.; Fak, J.J.; Nishiuchi, E.; Rice, C.M.; Darnell, R.B. miRNA-target chimeras reveal miRNA 3′-end pairing as a major determinant of Argonaute target specificity. Nat. Commun. 2015, 6, 8864. [Google Scholar] [CrossRef] [PubMed]
  117. Cai, Z.; Cao, C.; Ji, L.; Ye, R.; Wang, D.; Xia, C.; Wang, S.; Du, Z.; Hu, N.; Yu, X.; et al. RIC-seq for global in situ profiling of RNA-RNA spatial interactions. Nature 2020, 582, 432–437. [Google Scholar] [CrossRef] [PubMed]
  118. Martin, H.C.; Wani, S.; Steptoe, A.L.; Krishnan, K.; Nones, K.; Nourbakhsh, E.; Vlassov, A.; Grimmond, S.M.; Cloonan, N. Imperfect centered miRNA binding sites are common and can mediate repression of target mRNAs. Genome Biol. 2014, 15, R51. [Google Scholar] [CrossRef] [PubMed]
Insects 15 00491 g001
Figure 1. miRNA biogenesis and regulatory mechanism in Drosophila. Pri-miRNAs are transcribed by RNAPII in the nucleus and cleaved into pre-miRNAs by the microprocessor complex, which includes Drosha and Pasha. After pre-miRNAs are exported to the cytoplasm by Ranbp21, pre-miRNAs are further processed into miRNA duplex by Dicer-1. Finally, miRISC, containing a single-strand miRNA, suppresses the expression of specific genes by translation repression and/or mRNA degradation.
Figure 1. miRNA biogenesis and regulatory mechanism in Drosophila. Pri-miRNAs are transcribed by RNAPII in the nucleus and cleaved into pre-miRNAs by the microprocessor complex, which includes Drosha and Pasha. After pre-miRNAs are exported to the cytoplasm by Ranbp21, pre-miRNAs are further processed into miRNA duplex by Dicer-1. Finally, miRISC, containing a single-strand miRNA, suppresses the expression of specific genes by translation repression and/or mRNA degradation.
Insects 15 00491 g001
Insects 15 00491 g002
Figure 2. The roles of miRNAs involved in the developmental growth and apoptosis of Drosophila. (A) miR-276a, miR-8, and miR-14 mediate the regulation of the insulin/insulin-like growth factor signaling pathway. (B) Bantam, miR-14, miR-6, and miR-11 control the apoptosis signaling pathway.
Figure 2. The roles of miRNAs involved in the developmental growth and apoptosis of Drosophila. (A) miR-276a, miR-8, and miR-14 mediate the regulation of the insulin/insulin-like growth factor signaling pathway. (B) Bantam, miR-14, miR-6, and miR-11 control the apoptosis signaling pathway.
Insects 15 00491 g002
Insects 15 00491 g003
Figure 3. Involvement of miRNAs in the mushroom body (MB) development of Drosophila. Let-7 and miR-iab8 regulate the generation of MB neurons by controlling the transition of MB subtypes.
Figure 3. Involvement of miRNAs in the mushroom body (MB) development of Drosophila. Let-7 and miR-iab8 regulate the generation of MB neurons by controlling the transition of MB subtypes.
Insects 15 00491 g003
Insects 15 00491 g004
Figure 4. The signaling pathways regulated by miRNAs in wing development. (A) miR-5 and miR-960 control the Hh signaling pathway by targeting specific signaling component genes. (B) miR-7 and miR-252 regulate the Notch signaling pathway. (C) miR-31a/b and miR-8 are involved in the Wg signaling pathway.
Figure 4. The signaling pathways regulated by miRNAs in wing development. (A) miR-5 and miR-960 control the Hh signaling pathway by targeting specific signaling component genes. (B) miR-7 and miR-252 regulate the Notch signaling pathway. (C) miR-31a/b and miR-8 are involved in the Wg signaling pathway.
Insects 15 00491 g004
Insects 15 00491 g005
Figure 5. The roles of miRNAs in compound eye development of Drosophila. miR-7 and miR-279/996 regulate serial specification in the eye developmental process by modulating their target genes.
Figure 5. The roles of miRNAs in compound eye development of Drosophila. miR-7 and miR-279/996 regulate serial specification in the eye developmental process by modulating their target genes.
Insects 15 00491 g005
Table 1. Summary of development-associated miRNAs and their target genes in Drosophila.
Table 1. Summary of development-associated miRNAs and their target genes in Drosophila.
miRNATarget Gene Name
(Symbol)		Validation Methods 1Tissues/CellsReferencesSignaling Pathways
miR-252mushroom bodies tiny (mbt)Ago1 CLIP-seq, WB, Luc repFat body[58]-
Abelson interacting protein
(Abi)		Ago1 CLIP-seq, WB,
RT-qPCR, Luc rep		S2 cell[50]-
Rab6 (Rab6)Ago1 CLIP-seq, RT-qPCR, Luc repWing[59]Notch
miR-276aInsulin-like receptor (InR)Ago1 CLIP-seq, Luc repWing/fat body[60]IIS
nejire (nej)EGFP repNeuron[61]-
miR-8u-shaped (ush)RT-qPCR, WB, Luc repFat body[62]IIS
CG32767, wntless (wls)Luc repWing[63]Wg
miR-14sugarbabe (sug)Luc rep, EGFP repInsulin-producing neurosecretory cell[64]IIS
Death related ICE-like caspase (Drice)WBEye[65]Apoptosis
Bantamhead involution defective (hid) EGFP rep, ISWing[66]Apoptosis
brain tumor (brat),
prospero (pros)		RT-qPCR, Luc repNeuroblast[67]-
miR-6head involution defective (hid),
reaper (rpr), grim (grim),
sickle (skl)		RT-qPCR, Luc repCentral
nervous system		[68]Apoptosis
miR-11
let-7Chronologically inappropriate morphogenesis (chinmo)Luc rep, ISMushroom body[69]-
abrupt (ab)ISMushroom body[70]-
miR-iab8CG12229,
Ceramide phosphoethanolamine synthase (Cpes)		Behavioral analysesMushroom body[71]-
miR-92a/bJing interacting gene regulatory 1 (jigr1)RT-qPCR, IS, WB, Luc repNeuroblast[72]-
miR-124anachronism (ana)RT-qPCR, Luc repNeuroblast[73]-
saxophone (sax), wishful thinking (wit), thickveins (tkv), Mothers against dpp (Mad), Medea (Med)Luc repCentral
nervous system		[74]-
miR-34Neurexin IV (Nrx-IV),
hu li tai shao (hts)		ISCentral
nervous system		[75]-
miR-960smoothened (smo), costa (cos2),
fused (fu)		Luc rep, IS, EGFP repWing[76]Hh
miR-5smoothened (smo)Luc rep, EGFP rep, ISWing[77]Hh
miR-7Enhancer of split complex
(E(spl)-C)		EGFP repWing[78,79]Notch
Yan (=anterior open (aop))EGFP rep, ISEye[80]-
miR-31a/bwntless (wls)RT-qPCR, WBWing[81]Wg
miR-279/996rhomboid (rho), roughoid (ru),
bride of sevenless (boss)		EGFP rep, Luc repEye[82]-
1 WB, Western blotting; Luc rep, luciferase reporter assay; EGFP rep, EGFP reporter assay; IS, immunostaining.
Table 2. Sequencing techniques for identification of miRNA targets.
Table 2. Sequencing techniques for identification of miRNA targets.
Sequencing TechniquesFeatures 1Reference
RNA–Protein
interaction		HITS-CLIP- High-throughput CLIP-seq method using 254 nm UVC
- Identifies mRNA fragments and miRNAs associated with Ago protein
- Requires additional bioinformatic analysis to confirm miRNA–mRNA interactions		[110]
PAR-CLIP- Modified from HITS-CLIP
- Uses 4-thiouridine and 312–365 nm UVA/B to enhance RNA–protein crosslinking		[111]
iCLIP- Modified from HITS-CLIP
- Improves efficiency using DNA circularization after reverse transcription		[112]
eCLIP- Modified from HITS-CLIP
- Enhances efficiency using adapter ligation after reverse transcription		[113]
RNA–RNA
interaction		CLASH- Direct ligation of miRNA and mRNA fragments
- Includes Ago protein denaturation and two purification steps		[115]
CLEAR-CLIP- Direct ligation of miRNA and mRNA fragments
- Single purification step; does not require full denaturation of Ago		[116]
RIC-seq- Captures global RNA–RNA interactions using in situ proximity ligation with pCp-biotin
- May require Ago immunoprecipitation to enrich miRNA–mRNA interactions		[117]
1 It described only the basic characteristics and features of the method from the perspective of identifying miRNA targets.
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

Jang, D.; Kim, C.J.; Shin, B.H.; Lim, D.-H. The Biological Roles of microRNAs in Drosophila Development. Insects 2024, 15, 491. https://doi.org/10.3390/insects15070491

AMA Style

Jang D, Kim CJ, Shin BH, Lim D-H. The Biological Roles of microRNAs in Drosophila Development. Insects. 2024; 15(7):491. https://doi.org/10.3390/insects15070491

Chicago/Turabian Style

Jang, Daegyu, Chae Jeong Kim, Bo Hyun Shin, and Do-Hwan Lim. 2024. "The Biological Roles of microRNAs in Drosophila Development" Insects 15, no. 7: 491. https://doi.org/10.3390/insects15070491

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