Translator Disclaimer
1 December 2016 An RNAi Screen for Genes Involved in Nanoscale Protrusion Formation on Corneal Lens in Drosophila melanogaster
Author Affiliations +

The “moth-eye” structure, which is observed on the surface of corneal lens in several insects, supports anti-reflective and self-cleaning functions due to nanoscale protrusions known as corneal nipples. Although the morphology and function of the “moth-eye” structure, are relatively well studied, the mechanism of protrusion formation from cell-secreted substances is unknown. In Drosophila melanogaster, a compound eye consists of approximately 800 facets, the surface of which is formed by the corneal lens with nanoscale protrusions. In the present study, we sought to identify genes involved in “moth-eye” structure, formation in order to elucidate the developmental mechanism of the protrusions in Drosophila. We re-examined the aberrant patterns in classical glossy-eye mutants by scanning electron microscope and classified the aberrant patterns into groups. Next, we screened genes encoding putative structural cuticular proteins and genes involved in cuticular formation using eye specific RNAi silencing methods combined with the Gal4/UAS expression system. We identified 12 of 100 candidate genes, such as cuticular proteins family genes (Cuticular protein 23B and Cuticular protein 49Ah), cuticle secretion-related genes (Syntaxin 1A and Sec61 ββ subunit), ecdysone signaling and biosynthesis-related genes (Ecdysone receptor, Blimp-1, and shroud), and genes involved in cell polarity/cell architecture (Actin 5C, shotgun, armadillo, discs large1, and coracle). Although some of the genes we identified may affect corneal protrusion formation indirectly through general patterning defects in eye formation, these initial findings have encouraged us to more systematically explore the precise mechanisms underlying the formation of nanoscale protrusions in Drosophila.


Many insects possess a compound eye consisting of hundreds or thousands of ommatidial arrays. Each ommatidium comprises a set of photoreceptor cells, and its surface is covered with the corneal lens, through which light reaches the photoreceptive area, i.e., the rhabdom. Bernhard and Miller (1962) discovered that the outer surfaces of ommatidial lens are covered with an array of cuticular protrusions termed corneal nipples. The cone-shaped protrusions are 200–300 nm in height, and spaced in nearly hexagonal arrays. The nanoscale protrusion serves an anti-reflective function (Bernhard et al., 1963). Moreover, a recent study revealed that the self-cleaning property occurs due to the reduction of adhesive forces between contaminating materials and biological lens surfaces (Peisker and Gorb, 2010).

The corneal lens is one form of insect exoskeleton, the cuticle, and thus, the basic structure of lens is the same as that of the cuticle (Perry, 1968). The cuticle comprises a multi-layered structure, consisting of envelope, epicuticle, and procuticle (for review, see Locke, 2001). The outermost envelope functions to prevent water loss and is composed of proteins and lipids. Beneath it, the epicuticle functions to provide the stiffness of the cuticle and is composed of cross-linked proteins. The innermost procuticle confers elasticity to the cuticle and consists of chitin fiber-protein lattices. The formation of the multi-layered structure in the lens proceeds from the outermost to innermost layer (Gemne, 1971). Although the morphology and function of corneal protrusions have been studied, the molecular mechanism of nanoscale protrusion formation remains unclear.

In D. melanogaster, the nanoscale protrusions are also present on the lens surface of the ommatidia and ocelli (Stark et al., 1989). An ommatidium contains a set of eight photoreceptor cells, four cone cells, and two primary pigment cells, which is surrounded by three secondary pigment cells, three tertiary pigment cells, and three bristle cells. It is known that the cone cells and primary pigment cells secrete most components of the corneal lens, and secondary pigment cells also secrete corneal materials at the boundary between ommatidia (for review, see Charlton-Perkins and Cook, 2010). It has been reported that classical glossy eye fly mutants, such as glass (gl) (Stark and Carlson, 1991), lozenge (lz) (Stark and Carlson, 2000), and sparkling (spa) (Oster and Crang, 1972), possess aberrant “moth-eye” surfaces. Recently, atomic force microscopy (AFM) analysis of glossy eyes overexpressing Wingless showed a dramatic loss of corneal nano-structures (Kryuchkov et al., 2011). Thus, corneal nanoscale protrusions should be formed under genetic regulation. Given the availability of many powerful genetic tools, D. melanogaster thus is an excellent insect model for investigating the developmental mechanisms that give rise to corneal protrusions.

In the present study, we sought to identify genes involved in the formation of corneal nanoscale protrusions as a means to begin to elucidate the mechanism in Drosophila. A better understanding of this phenomenon would allow us to more fully appreciate the intricate landscape of the ordered nanoscale structures using the genetically amenable fruit fly, to contribute to the field of self-organization of secreted substances from cells in developmental biology, and to adapt novel bioengineering methods to the creation of bioinspired applications, such as anti-reflective and self-cleaning functions, inspired by the “moth-eye” structure.


Fly stocks and crossings for screening

All flies were reared on yeast-glucose-cornmeal-agar medium at 25°C. Canton-Special (CS) flies were used as wild-type controls. Four classical glossy-eye mutants, Glazed (Gla: a dominant allele of wingless), lz3, gl1, and spapol were obtained from the Bloomington stock center and Kyoto Stock Center. In our screen to identify genes involved in the corneal nanoscale protrusion formation, the RNAi-mediated knockdown of a gene was induced using the Gal4/UAS system (Brand and Perrimon, 1993). UAS-RNAi transgenic fly lines were obtained from the Vienna Drosophila Resource Center (VDRC) and the National Institute of Genetics (NIG) RNAi stocks. The information is summarized in  Supplementary Tables S1 and S2 online (10.2108.zsj.33.583.s1.pdf). These RNAi lines were crossed with an eye-specific Gal4 driver, GMR-Gal4, which expresses Gal4 under the control of glass multiple reporter (GMR) promoter elements (from Bloomington stock center), and the corneal protrusion patterns of F1 progeny were examined using a scanning electron microscope (SEM). When the F1 progeny showed lethality at the pharate adult stage, pharate adults were dissected out of the puparium, the pupal cuticle was removed, and then the corneal protrusion patterns were examined, if possible.

Scanning electron microscopy

Adult female flies were fixed for 30 min in 3.7% formaldehyde in PBS-0.006% TritonX-100, washed once for 15 min in PBS-0.3% TritonX-100, twice for 15 min in distilled water, and serially dehydrated with 25%, 50%, 75%, and 90% ethanol for more than 15 min and with 100% ethanol overnight. After dehydration, ethanol was replaced with 50% tert-butyl alcohol for 15 min and then twice with 100% tert-butyl alcohol for 30 min. Then, the sample was frozen at 4°C for 15 min. Finally, flies were further dehydrated by freeze-drying using a freeze dryer (VFD-21S, Vacuum Device Inc). Specimens were subjected to gold-coating by an ion coater (Neo coater MP-19010 NCTR, JEOL), and the corneal lens was observed using a SEM (TM3000 Miniscope, Hitachi).


Corneal protrusion patterns in Drosophila

The Drosophila compound eye is composed of approximately 800-unit facets or ommatidia that arranged in a precise hexagonal array (Fig. 1A). Hair-like structures called interommatidial bristles are present between the ommatidial lenses (Fig. 1A'). Cone-shaped nanoscale protrusions exist on the surface of the corneal lens (Fig. 1A'), and the protrusions are arranged in an approximately regular hexagonal close-packed pattern (Fig. 1A”). We also observed nanoscale protrusions with number of five or seven nearest neighbors in wild type flies. According to our measurement by SEM, the distance adjacent to the tip of the protrusions was about 250 nm in wild type flies, which corroborates previous AFM studies (Kryuchkov et al., 2011).

Aberrant corneal protrusion patterns in classical glossy-eye mutants

We observed the corneal surface patterns in four classical viable mutants, Gla, lz3, gl1, and spapol, with glossy eyes by SEM, and typical features of aberrant patterns of corneal protrusions in the mutants were classified (Fig. 1B”-E”). The ommatidial lens of Gla mutants had a flat surface (Fig. 1B), and the nanoscale protrusions were either not evident or diminished in these lens surfaces (no-protrusion type; Fig. 1B' and B”). The genes lz, spa, and gl are known to encode transcription factors crucial for pre-patterning photoreceptor precursors (Daga et al., 1996) and photoreceptor cell development (Fu and Noll, 1997; Moses et al., 1989). Loss-of-function mutant alleles lz3, gl1, and spapol displayed small ommatidial sizes, irregular alignment, and defects of the dome shape in the corneal lens (Fig. 1C-E and C'-E'). We observed the grainy cuticle structure in lz3 ommatidial surface (grainy type; Fig. 1C”). In gl1 and spapol mutants, we observed elongated protrusions, which suggested that some nanoscale protrusions were fused in the ommatidial surface (fusion type; Fig. 1D” and E”). There were also maze-like structures in the spapol mutant (maze type; Fig. 1E”). The maze type may arise from many fused protrusions connected over a wide range. In addition, nanoscale protrusions disappeared partially in lens of the lz3, gl1, and spapol mutants (Fig. 1C', D' and E'). In addition to the four phenotypes categorized in the classical glossy-eye mutants, we have identified another type of aberrant protrusion whose size is larger than that of wild type (enlarged type; Fig. 1F-F”, see below). Thus, we recognize five aberrant protrusion patterns in total.

Screening of the candidate genes functioning in corneal protrusion formation

To elucidate the molecular and cellular mechanisms of the nanoscale protrusion formation, we carried out RNAi screening of genes in which their knockdowns induced aberration of corneal protrusion formation. Specifically, we induced RNAi in candidate genes with the eye specific GMR-Gal4 driver and observed corneal protrusion patterns in these flies. We focused on two types of candidate genes: cuticular protein (CPR) family genes, and genes involved in cuticular formation. There are 102 putative CPR family genes, which are characterized by a conserved region known as the chitin-binding Rebers and Riddiford Consensus (R&R Consensus) (Cornman, 2009). The functions of most CPR family genes remain unknown. In this study, we screened 68 CPR family genes (107 RNAi lines) ( Supplementary Table S1 (10.2108.zsj.33.583.s1.pdf)) and identified two genes, Cpr23B and Cpr49Ah, which were crucial for proper corneal protrusion formation (Table 1). We then investigated the influence of RNAi knockdown of genes that affect the cuticle development of the body surface at the embryonic, larval, and adult phases. These genes belong to five categories: chitin assembly, sclerotization and melanization, secretion, ecdy ecdysone signaling, and cell polarity (Schwarz and Moussian, 2007). We screened 32 genes from these five categories and identified 10 genes crucial for corneal protrusion formation ( Supplementary Table S2 (10.2108.zsj.33.583.s1.pdf)). Overall, we identified 12 genes (Table 1) out of 100 candidate genes. The effects of RNAi knockdown and impact on corneal protrusion formation for each category are detailed in the following sections.

Fig. 1.

Scanning electron micrograph of six types of corneal protrusion patterns in wild-type flies, classical glossy-eye mutants and Act5C knockdown flies. (A-A”) wild-type flies CS (normal type). (B-B”) y1 w67c23; In(2LR)Gla, wgGla-1/SM6a (no-protrusion type). (C-C”) lz3 (grainy type). (D-D”) gl1 (fusion type). (E-E”) spapol (maze type). (F-F”) w; GMR-Gal4/UAS-Act5C RNAi (HMS02487) (enlarged type). Scale bars: 300 µm (A-F), 10 µm (A'-F'), 1 µm (A”-F”).


Cuticular protein (CPR) family genes

RNAi-mediated knockdown of Cpr23B and Cpr49Ah that resulted in the reduction of the activity of two genes induced aberrant protrusion formation. In these knockdown flies, we frequently observed glossy and rough compound eyes with fused ommatidia (Fig. 2A and B). Corneal protrusions of Cpr23B knockdown flies were enlarged (Fig. 2A' white arrowhead), while the Cpr49Ah knockdown flies had maze type and grainy type protrusions (Fig. 2B' black arrow and open white arrowhead, respectively). Additionally the protrusions disappeared partially at the margin of the corneal lens in Cpr23B and Cpr49Ah knockdown flies (Fig. 2A' and B' asterisks).

The roles of Cpr23B and Cpr49Ah genes were not well known with regards to cuticle formation. One recent study reported that a mutation of Cpr49Ah resulted in thin and misaligned wing hair phenotypes (Adler et al., 2013). Hence, the Cpr49Ah is also required for proper cuticle formation of the lens, as well as the wing hair.

Genes involved in cuticular formation

Chitin assembly

The procuticle is composed of a protein-chitin matrix that confers elasticity to the cuticle. Chitin's composition of β 1,4- linked N-acetylglucosamine (GlcNAc) keenly contributes to the arthropod exoskeleton (for review, see Muthukrishnan et al., 2012). GlcNAc is converted into activated monomers by the uridine diphosphate (UDP)-GlcNAc pyrophosphorylase encoded by the mummy (mmy) gene (Araújo et al., 2005), and chitin fibers are synthesized by Chitin Synthase-1 encoded by the krotzkopf verkehrt (kkv) gene (Moussian et al., 2005a). The chitin fibers protrude into the extracellular space, where the chitin-protein complex is organized. Apical membrane-anchored extracellular proteins, encoded by the retroactive (rtv) and knickkopf (knk) genes, play an important role in organizing and orientating chitin fibers (Moussian et al., 2005b; Moussian et al., 2006). Another membrane-associated protein encoded by piopio (pio) has been shown to be required for attachment of the procuticle to the apical epidermal surface (Bökel et al., 2005). In addition to membrane-associated factors, apical extracellular matrix chitin deacetylase proteins, encoded by the vermiform (verm) and serpentine (serp) genes, function in the organization and orientation of chitin fibers (Luschnig et al., 2006). Moreover, Schlaff (encoded by slf) is one of the unidentified factors affecting cuticle differentiation and structure (Nüsslein-Volhard et al., 1984).

Table 1.

Effects of RNAi knockdown of the candidate genes on protrusion formation.


Fig. 2.

Scanning electron micrograph of corneal protrusion patterns in Cpr knockdown flies. (A, A') w/UAS-Cpr23B RNAi 2973R-1; GMR-Gal4/+. (B, B') w; GMR-Gal4/+; UAS-Cpr49Ah RNAi 8515R-1/+. White arrowhead in (A'): enlarged type. Asterisks in (A') and (B'): the protrusions disappeared partially at the margin (no-protrusion type). Open white arrowhead in (B'): grainy type. Black arrow in (B'): maze type. Scale bars: 300 µm (A, B), 10 µm (A', B').


We examined the effect of RNAi-mediated knockdown of these eight genes on corneal protrusion formation. We did not detect any aberrations of the protrusion pattern in flies with knockdowns of mmy, knk, rtv, serp, verm, slf, and pio genes ( Supplementary Table S2 (10.2108.zsj.33.583.s1.pdf)). The effect of kkv knockdown could not be examined, because kkv knockdown was lethal at the pharate adult stage, and the surface of their eyes was often ruptured and melanized. Mutant embryos for kkv, which lose chitin in the cuticle, have been shown in previous studies to display abnormally soft cuticles with poor mechanical integrity (Moussian et al., 2005a). Likewise, loss of corneal chitin should cause similar defects in lens formation. Thus, in our screening, most of chitin biosynthesis factors do not directly affect the formation of protrusion pattern. Chitin defects induced in the procuticle layer may not affect the envelope and epicuticle layers where corneal protrusion formation proceeds. However, we note that our RNAi knockdown system may be insufficiently powerful to induce corneal protrusion defects.

Sclerotization and melanization

Cuticle differentiation requires the process of hardening (sclerotization) and tanning (melanization), which are induced by some catecholamine metabolites with related proteins and enzymes. Tyrosine is converted into dopa by the enzyme tyrosine hydroxylase encoded by the pale (ple) gene (Neckameyer and White, 1993), and dopa is subsequently converted into dopamine by dopa decarboxylase, encoded by the Dopa decarboxylase (Ddc) gene (Bishop and Wright, 1987), or into N-β-alanyl dopamine (NBAD) by β-alanyl dopamine synthase encoded by the ebony (e) gene (Richardt et al., 2003). These catecholamines which are synthesized in epidermal cells are released into cuticle layers as precursors for sclerotization and melanization, in which phenol oxidase catalyzes them into their respective quinone derivatives. Quinones such as NBAD-quinone bind covalently to cuticlar proteins that function in cuticle sclerotization. Dopa- and dopamine-quinones are converted to melanogenic substrates through the enzymatic activity of Ebony encoded by the ebony (e) gene, aspartate decarboxylase encoded by the black (b) gene (Phillips et al., 2005), NBAD hydrolase encoded by the tan (t) gene (True et al., 2005), and carboxypeptidase D (CPD) encoded by the silver (svr) gene (Settle et al., 1995). Additionally, the yellow (y) gene is known to be involved in cuticle melanization (Riedel et al., 2011).

We examined the effect of knockdown in the pale, Ddc, e, b, t, svr, and y on corneal protrusion formation (12 RNAi lines). No aberrant protrusion formations were observed in these knockdown flies ( Supplementary Table S2 (10.2108.zsj.33.583.s1.pdf)). This result is plausible because no pigmentation occurs in lens cuticle, and sclerotization would proceed after corneal protrusion formation. Usually, after eclosion, secretion of the bursicon hormone causes sclerotization, whereas corneal protrusion formation occurs during the middle of the pupal stage in the fruit fly (Yamahama and Kimura, unpublished data) as well as the moth, Manduca sexta (Gemne, 1971). Thus, the factors for cuticular sclerotization and melanization are not involved in corneal protrusion formation.


Recently, secretion mechanisms in cuticle differentiation have been investigated (Valcárcel et al., 1999; Abrams and Andrew, 2005; Moussian et al., 2007). We examined the effect of knockdown on corneal protrusion formation in seven cuticle secretion-related genes: Syntaxin 1A (Syx1A) which codes for a product that interacts with the soluble N-ethylmaleimide-sensitive factor attachment protein receptor (SNARE) (Schulze et al., 1995); Sec61 β subunit (Sec61β ) which encodes a subunit of Sec61 endoplasmic reticulum (ER) translocon protein (Valcárcel et al., 1999); Coat Protein γ (γ COP) gene that encodes a subunit of the Coat Protein Complex (COP) I coatomer complex, which is trafficked primarily from the early Golgi to the endoplasmic reticulum (ER) (Abrams and Andrew, 2005); and Sar1, Sec31, haunted (hau: Sec23) and ghost (gho) genes which collectively encode component proteins of the COP II complex that mediates protein transport from the ER to Golgi (Norum et al., 2010). Out of the seven genes examined, RNAi knockdown of two genes, Syx1A and Sec61β induced severe defects in corneal protrusion formation ( Supplementary Table S2 (10.2108.zsj.33.583.s1.pdf)). Ommatidia in Syx1A knockdown flies were frequently fused and decreased in size, especially at the posterior region of the eye (Fig. 3A). Protrusions on the corneal lens were enlarged at the center and disappeared at the margin (Fig. 3A' white arrowhead and asterisks) and frequently fused to form a line (Fig. 3A' white arrow). Moreover, there were grainy structures (Fig. 3A' open white arrowheads). In Sec61β knockdown ommatidia, protrusions disappeared at the margin of the lens (Fig. 3B and B' asterisks) and were unequally distributed at the center of the lens where protrusions appeared to be irregular in size (Fig. 3B' white arrowhead). Thus, defects of protein trafficking affect corneal protrusion formation, a finding that is further supported by the fact that the protein epicuticle layer, in which protrusions are formed in the corneal lens, is absent in Drosophila Sec61β mutant embryos (Valcárcel et al., 1999). The corneal protrusion pattern in Sec31 knockdown ommatidia appeared to be normal (data not shown). Sar1, γ COP, hau, and gho knockdown flies could not be examined because they were lethal during the pharate adult stage and possessed fragile lens (data not shown) like the kkv knockdown flies. The membrane vesicle trafficking via COP I and COP II is a major secretory route responsible for full cuticle differentiation (Abrams and Andrew, 2005; Norum et al., 2010). To investigate the effects of those lethal genes on corneal protrusion formation, we will consider using a weak Gal4-driver line to induce RNAi or hypomorphic mutations.

Fig. 3.

Scanning electron micrograph of corneal protrusion patterns in flies with RNAi knockdown of genes involved in cuticle secretion. (A, A') w; GMR-Gal4/UAS-Syx1A RNAi R-3. (B, B') w; GMR-Gal4/+; UAS-Sec61β RNAi 8785/+. Open white arrowheads in (A'): grainy type. White arrowheads in (A') and (B'): enlarged type. Asterisks in (A') and (B'): the protrusions disappeared partially at the margin (no-protrusion type). White arrow in (A'): fusion type. Scale bars: 300 µm (A, B), 10 µm (A', B').


Ecdysone signaling

In Drosophila, ecdysteroids, including ecdysone and its derivative 20-hydroxyecdysone (20E), are important for cuticle formation (Doctor et al., 1985). Response to ecdysteroids are mediated by a functional Ecdysone receptor (EcR)/Ultraspiracle (Usp) heterodimer (Thomas et al., 1993; Yao et al., 1993). Moreover, the 20E is known to directly induce the B lymphocyte-induced maturation protein 1 (Blimp-1) gene which regulates the timing of the ecdysone-induced developmental pathway (Agawa et al., 2007).

We assessed the effect of gene knockdown in two ecdysone signaling genes, EcR and Blimp-1Supplemetary Table S2 (10.2108.zsj.33.583.s1.pdf)). We observed abnormalities at the center region of the compound eye upon the knockdown of EcR and Blimp-1 (Fig. 4A and B). In EcR knockdown corneal lens, the fused protrusions merged into a maze at the center region (Fig. 4A' black arrow) and the periphery contained a partial loss of protrusions (Fig. 4A' asterisks). Moreover, huge grainy protrusions surrounded at the outermost region (Fig. 4A' open white arrowheads). We observed the fusion type and grainy type as a weak phenotype of the EcR knockdown at the center region of the lens (data not shown). Blimp-1 knockdown lens also showed no protrusions and a rough surface (Fig. 4B' asterisk). It has been suggested that there is a relationship between ecdysone signaling and secretion of the cuticle. It was reported that ecdysone induces Golgi formation by driving the transcription of a number of genes coding for factors of the ER and Golgi, such as the COP II component Sec23 in the imaginal discs (Dunne et al., 2002; Kondylis et al., 2001). These findings suggest that secretion and membrane trafficking may be a fundamental response to the hormone pulse.

The genes involved in ecdysone biosynthesis are known as Halloween-group genes, mutations of which cause loss of ecdysone during embryogenesis, resulting in cuticle differentiation defects (Chávez et al., 2000). We examined the gene-silencing effect of one of the Halloween-group genes, shroud (sro), which encodes a short-chain dehydrogenase/reductase (Niwa et al., 2010). We often observed fused ommatidia in sro knockdown flies (Fig. 4C). The corneal protrusions were irregular in size (Fig. 4C' white arrowhead) and of the grainy type (Fig. 4C' open white arrowhead). In the pupal stage, ecdysone and its derivative 20E are secreted from the gland cells into the hemolymph and act on the epidermis to regulate cuticle formation. Since sro gene-knockdown is induced only within the ommatidial cell, this effect on corneal protrusions may not be caused by ecdysone directly. Sro is a member of the Short-chain dehydrogenase/reductase enzymes, which play roles in lipid, amino acid, carbohydrate, cofactor, and hormone metabolism in a wide range of cells and tissues (Kavanagh et al., 2008). Therefore, the sro gene might have some unknown function in corneal lens cuticle formation besides ecdysteroid biosynthesis.

Fig. 4.

Scanning electron micrograph of corneal protrusion patterns in flies with RNAi knockdown of genes involved in ecdysone signaling and biosynthesis. (A, A') w; GMR-Gal4/UAS-EcR RNAi 9327. (B, B') w; GMR-Gal4/+; UAS-blimp-1 RNAi R-2/+. (C, C') w; GMR-Gal4/+; UAS-sro RNAi 16386/+. Open white arrowheads and black arrow in (A'): grainy type and maze type, respectively. Asterisks in (A', B'): the protrusions disappeared partially at the margin (no-protrusion type). Open white arrowhead in (C'): grainy type. White arrowhead in (C'): enlarged type. Scale bars: 300 µm (A-C), 10 µm (A'-C').


Cell polarity/cell architecture

Cell polarity provides information for the correct localization of certain factors to the apical plasma membrane for secretion of cuticle material to the extracellular matrix. One of the planar cell polarity genes Drosophila E-cadherin (DE-cadherin), encoded by the shotgun (shg) gene, is required for proper embryonic cuticle development (Tepass et al., 1996). DE-cadherin forms a complex with α-catenin encoded by the α -cat gene, β-catenin encoded by the armadillo (arm) gene, and adherens junction (AJ) protein p120, which is collectively called the cadherin/catenin complex. This cadherin/catenin complex binds to filamentous actin, and is essential in proper cell adhesion (Pai et al., 1996). The crumbs (crb) gene encodes a large transmembrane protein required for maintenance of apico-basal cell polarity and AJ in embryonic epithelia (Tepass et al., 1990; Tepass and Knust, 1990). Moreover, insects have a semi-permeable barrier that called the septate junctions (SJ) at basal region of the AJ. Two genes, discs large 1 (dlg1) and coracle (cora), are well known as SJ component genes (Woods and Bryant, 1993; Fehon et al., 1994). These genes are involved in cell polarity and serve as factors that maintain the cellular architecture.

We investigated the effect in these six genes on corneal protrusion formation: shg, arm, crb, dlg1, cora, and cytoskeletal actin gene (Act5C) ( Supplementary Table S2 (10.2108.zsj.33.583.s1.pdf)). Five of the six genes silenced resulted in abnormal protrusion formation. We observed fused ommatidia in Act5C, shg, and arm knockdown flies (Fig. 5A-C). In particular, these flies exhibited enlarged protrusions (Fig. 5A'-C' white arrowheads) and occasionally had fused protrusions and grainy structures (Fig. 5A'-C' white arrows and open white arrowheads). In addition, in shg knockdown flies, protrusions partially disappeared at the lens surface margin (Fig. 5B' asterisks). The protrusion pattern in crb knockdown ommatidia, in contrast, appeared normal (data not shown). Interestingly, common effects of protrusion enlargement were induced by aberration of the cadherin/catenin complex. This implies that cell polarity or cell architecture regulated by intercellular adhesion and actin-based cytoskeleton controls the size of protrusions during its formation.

The dlg1 knockdown flies possessed small compound eye sizes and defects of the dome shape in the ommatidial corneal lens (Fig. 5D). The protrusions disappeared partially at the margin in the ommatidia of dlg1 knockdown flies as well (Fig. 5D' asterisks). Alternatively, cora knockdown eyes, the ommatidial alignment of which appeared to be normal, showed loss of protrusions at the center of the lens (Fig. 5E and E' asterisk). Although it is interesting that dlg1 and cora knockdowns affect the reciprocal region, the cause of these phenotypes remains unclear.

We have shown that corneal protrusion formation is under the genetic control of various genes, and that these genes can be modulated to impact the dynamics of protrusion formation. However, it is important to consider that protrusion defects may be mediated by more general defects in eye patterning prior to protrusion formation. The genes identified here may affect corneal protrusion formation indirectly through general patterning defects in eye formation. Certainly, some genes, such as arm, dlg and cora, are known to be involved in eye patterning (Ahmed et al., 1998; Beronja et al., 2005; Legent et al., 2012; Lamb et al., 1998). Assessments of whether and how the respective genes are expressed in the lens-secreting cells at the time of protrusion formation would help to address whether the effects are direct or indirect. Additionally, we note two technical limitations of the RNAi knockdown approached used in this study. We did not control for the effectiveness of the RNAi constructs used to down-regulate the respective genes. Examining for the expression levels of the respective genes would be helpful to confirm the function of the gene in protrusion formation. In addition, we cannot rule out the possibility that some of the RNAi phenotypes were caused by off-target effects.

Various corneal protrusion patterns are observed in nature (Sukontason et al., 2008). Moreover, Blagodatski et al. (2015) provides a comprehensive analysis of the corneal protrusion pattern in 23 insect orders, some of which were similar to patterns resulting from gene knockdowns in our study, e.g., irregular protrusions of various sizes, strands merging into a maze, and observations of maze-like structures. These findings imply that evolutionary diversification of insect corneal protrusion patterns results from species-specific modification of gene regulation involved in corneal protrusion formation.

Fig. 5.

Scanning electron micrograph of corneal protrusion patterns in flies with RNAi knockdown of genes involved in cell polarity/cell architecture. (A, A') w; GMR-Gal4/CyO; UAS-Act5C RNAi (HMS02487)/TM6,Tb. (B, B') w; GMR-Gal4/UAS-shg RNAi R-3. (C, C') w; GMR-Gal4/UAS-arm RNAi R-1. (D, D') w; GMR-Gal4/UAS-dlg1 RNAi R-2. (E, E') w; GMR-Gal4/UAS-cora RNAi 9787. White arrows, open white arrowheads and white arrowheads in (A', B', C'): fusion type, grainy type and enlarged type, respectively. Asterisks in (B', D') (at the margin) and E'(at the center): no-protrusion type. Scale bars: 300 µm (A-E), 10 µm (A'-E').


In corneal protrusion formation, Gemne (1971) proposed that the corneal protrusions originate from secretion by the regularly spaced microvilli of the cone lens cells by observing protrusion formation using transmission electron microscopy (TEM) in Manduca. Blagodatski et al. (2015) reported a rich diversity of insect corneal protrusion patterns among which transitions appeared, sometimes within the same lens, and suggested that formation on the tip of microvilli is not satisfactory to account for nanoscale protrusions. They proposed an alternative mathematical model based on the Turing reaction-diffusion mechanism, and were able to simulate various protrusion patterns found in nature. They hypothesized that the Turing reaction-diffusion mechanism for nanoscale protrusion pattern formation is mediated by organic components of the lens, possessing different diffusion properties and mutually influencing each other's abundance, polymerization, and aggregation. Although the molecular identity of the components or morphogens patterning corneal protrusions remains unknown, our studies may provide some insights into the components. For instance, knockdown of two CPR genes may provide potential insight about the materials needed for lens formation based on our phenotypes observed in our RNAi screening. Hence, these CPR genes might encode one of the components related to the Turing reaction-diffusion processes. In addition, we found that various corneal protrusion phenotypes are present on identical lens surfaces in RNAi knockdown flies. The expression level of Gal4 in the GMR-Gal4 line was not uniform among lens-producing cells at the pupal protrusion formation stage, if membrane-bound GFP was driven (data not shown). Thus, mixed phenotypes on one lens may result from differences in the effects of RNAi-mediated knockdown in different lens-producing cells.

Interestingly, gene knockdown of cellular actin also influenced corneal protrusion formation in our screening. The microvillus core is composed of actin (Gemne, 1971), and the change of corneal protrusion patterns might therefore have been caused by defective microvilli. Even if the Turing mechanism does act in the formation of nanoscale protrusions as suggested by Blagodatski et al. (2015), microvilli may nonetheless act as the first scaffolds for this reaction. To test this hypothesis, we must examine the formative process of various protrusion patterns chronologically in mutants which were identified in this study.

“Moth-eye” structure-like corneal protrusions, which serve anti-reflective, self-cleaning, and/or water-repellent functions, has emerged at the forefront of nature-inspired biomimetic technology. While morphology and function of “moth-eye” structure are relatively studied as discussed earlier (Bernhard and Miller, 1962; Bernhard et al., 1963), the mechanism of the formation is still elusive. However, our initial attempts to identify the factors involved in the nanoscale protrusion formation on the corneal lens using the model insect, D. melanogaster, have encouraged us to further examine the precise mechanisms regulating nanoscale protrusion formations. Elucidation of the mechanism will inspire us to develop “moth-eye”-inspired nanostructured products.


We thank Kyoto Stock Center, NIG-FLY stock center, Bloomington Stock Centers and Vienna Drosophila RNAi Center for numerous Drosophila strains; H. Fudouji, S. Yoshioka, D. Ishii, M. Shimomura and Y. Uozu for valuable discussion; and A. Izumi for technical assistance. This work was supported by a Grant-in-Aid for Scientific Research on Innovative Areas from the Ministry of Education, Culture, Sports, Science and Technology (MEXT) of Japan to K-I. K., H. K and T. H. (No. 24120004).


  1. Abrams EW, Andrew DJ ( 2005) CrebA regulates secretory activity in the Drosophila salivary gland and epidermis. Development 132: 2743–2758  Google Scholar

  2. Adler PN, Sobala LF, Thom D, Nagaraj R ( 2013) dusky-like is required to maintain the integrity and planar cell polarity of hairs during the development of the Drosophila wing. Dev Biol 379: 76–91  Google Scholar

  3. Agawa Y, Sarhan M, Kageyama Y, Akagi K, Takai M, Hashiyama K, et al. ( 2007) Drosophila Blimp-1 is a transient transcriptional repressor that controls timing of the ecdysone-induced developmental pathway. Mol Cell Biol 27: 8739–8747  Google Scholar

  4. Ahmed Y, Hayashi S, Levine A, Wieschaus E ( 1998) Regulation of Armadillo by a Drosophila APC inhibits neuronal apoptosis during retinal development. Cell 93:1171–1182  Google Scholar

  5. Araújo SJ, Aslam H, Tear G, Casanova J ( 2005) mummy/cystic encodes an enzyme required for chitin and glycan synthesis, involved in trachea, embryonic cuticle and CNS development-Analysis of its role in Drosophila tracheal morphogenesis. Dev Biol 288: 179–193  Google Scholar

  6. Bernhard CG, Miller WH ( 1962) A corneal nipple pattern in insect compound eyes. Acta Physiol Scand 56: 385–386  Google Scholar

  7. Bernhard CG, William HM, Aage RM ( 1963) Function of the corneal nipples in the compound eyes of insects. Acta Physiol Scand 58: 381–382  Google Scholar

  8. Beronja S, Laprise P, Papoulas O, Pellikka M, Sisson J, Tepass U ( 2005) Essential function of Drosophila Sec6 in apical exocytosis of epithelial photoreceptor cells. J Cell Biol 169: 635–646  Google Scholar

  9. Bishop CP, Wright TR ( 1987) DdcDE1, a mutant differentially affecting both stage and tissue specific expression of dopa decarboxylase in Drosophila. Genetics 115: 477–491  Google Scholar

  10. Blagodatski A, Sergeev A, Kryuchkov M, Lopatina Y, Katanaev VL ( 2015) Diverse set of Turing nanopatterns coat corneae across insect lineages. Proc Natl Acad Sci USA 112: 10750–10755  Google Scholar

  11. Bökel C, Prokop A, Brown NH ( 2005) Papillote and Piopio: Drosophila ZP-domain proteins required for cell adhesion to the apical extracellular matrix and microtubule organization. J Cell Sci 118: 633–642  Google Scholar

  12. Brand AH, Perrimon N ( 1993) Targeted gene expression as a means of altering cell fates and generating dominant phenotypes. Development 118: 401–415  Google Scholar

  13. Charlton-Perkins M, Cook TA ( 2010) Building a fly eye: Terminal differentiation events of the retina, corneal lens, and pigmented epithelia. Curr Top Dev Biol 93: 129–173  Google Scholar

  14. Chávez VM, Marqués G, Delbecque JP, Kobayashi K, Hollingsworth M, Burr J, et al. ( 2000) The Drosophila disembodied gene controls late embryonic morphogenesis and codes for a cytochrome P450 enzyme that regulates embryonic ecdysone levels. Development 127: 4115–4126  Google Scholar

  15. Cornman RS ( 2009) Molecular evolution of Drosophila cuticular protein genes. PLoS ONE 4: e8345 Google Scholar

  16. Daga A, Karlovich CA, Dumstrei K, Banerjee U ( 1996) Patterning of cells in the Drosophila eye by Lozenge, which shares homologous domains with AML1. Genes Dev 10: 1194–1205  Google Scholar

  17. Doctor J, Fristrom D, Fristrom JW ( 1985) The pupal cuticle of Drosophila: biphasic synthesis of pupal cuticle proteins in vivo and in vitro in response to 20-hydroxyecdysone. J Cell Biol 101: 189–200  Google Scholar

  18. Dunne JC, Kondylis V, Rabouille C ( 2002) Ecdysone triggers the expression of Golgi genes in Drosophila imaginal discs via Broad-complex. Dev Biol 245: 172–186  Google Scholar

  19. Fehon RG, Dawson IA, Artavanis-Tsakonas S ( 1994) A Drosophila homologue of membrane-skeleton protein 4. 1 is associated with septate junctions and is encoded by the coracle gene. Development 120: 545–557  Google Scholar

  20. Fu W, Noll M ( 1997) The Pax2 homolog sparkling is required for development of cone and pigment cells in the Drosophila eye. Genes Dev 11: 2066–2078  Google Scholar

  21. Gemne G ( 1971) Ontogenesis of corneal surface ultrastructure in nocturnal Lepidoptera. Phil Trans Roy Soc Lond B 262: 343–363  Google Scholar

  22. Kavanagh KL, Jörnvall H, Persson B, Oppermann U ( 2008) Medium- and short-chain dehydrogenase/reductase gene and protein families: The SDR superfamily: functional and structural diversity within a family of metabolic and regulatory enzymes. Cell Mol Life Sci 65: 3895–3906  Google Scholar

  23. Kondylis V, Goulding SE, Dunne JC, Rabouille C ( 2001) Biogenesis of Golgi stacks in imaginal discs of Drosophila melanogaster. Mol Biol Cell 12: 2308–2327  Google Scholar

  24. Kryuchkov M, Katanaev VL, Enin GA, Sergeev A, Timchenko AA, Serdyuk IN ( 2011) Analysis of micro- and nano-structures of the corneal surface of Drosophila and its mutants by atomic force microscopy and optical diffraction. PLoS ONE 6: e22237 Google Scholar

  25. Lamb RS, Ward RE, Schweizer L, Fehon RG ( 1998) Drosophila coracle, a member of the protein 4.1 superfamily, has essential structural functions in the septate junctions and developmental functions in embryonic and adult epithelial cells. Mol Biol Cell 9: 3505–3519  Google Scholar

  26. Legent K, Steinhauer J, Richard M, Treisman JE ( 2012) A screen for x-linked mutations affecting Drosophila photoreceptor differentiation identifies casein kinase 1α as an essential negative regulator of wingless signaling. Genetics 190: 601–616  Google Scholar

  27. Locke M ( 2001) The Wigglesworth Lecture: Insects for studying fundamental problems in biology. J Insect Physiol 47: 495–507  Google Scholar

  28. Luschnig S, Bätz T, Armbruster K, Krasnow MA ( 2006) serpentine and vermiform encode matrix proteins with chitin binding and deacetylation domains that limit tracheal tube length in Drosophila. Curr Biol 16: 186–194  Google Scholar

  29. Moses K, Ellis MC, Rubin GM ( 1989) The glass gene encodes a zinc-finger protein required by Drosophila photoreceptor cells. Nature 340: 531–536  Google Scholar

  30. Moussian B, Schwarz H, Bartoszewski S, Nüsslein-Volhard C ( 2005a) Involvement of chitin in exoskeleton morphogenesis in Drosophila melanogaster. J Morphol 264: 117–130  Google Scholar

  31. Moussian B, Söding J, Schwarz H, Nüsslein-Volhard C ( 2005b) Retroactive a membrane-anchored extracellular protein related to vertebrate snake neurotoxin-like proteins, is required for cuticle organization in the larva of Drosophila melanogaster. Dev Dyn 233: 1056–1063  Google Scholar

  32. Moussian B, Seifarth C, Müller U, Berger J, Schwarz H ( 2006) Cuticle differentiation during Drosophila embryogenesis. Arthropod Struct Dev 35: 137–152  Google Scholar

  33. Moussian B, Veerkamp J, Müller U, Schwarz H ( 2007) Assembly of the Drosophila larval exoskeleton requires controlled secretion and shaping of the apical plasma membrane. Matrix Biol 26: 337–347  Google Scholar

  34. Muthukrishnan S, Merzendorfer H, Arakane Y, Kramer KJ ( 2012) Chitin metabolism in insects. In “Insect Molecular Biology and Biochemistry” Ed by LI Gilbert, Academic Press, San Diego, pp 193–235 Google Scholar

  35. Neckameyer WS, White K ( 1993) Drosophila tyrosine hydroxylase is encoded by the pale locus. J Neurogenet 8: 189–199  Google Scholar

  36. Niwa R, Namiki T, Ito K, Shimada-Niwa Y, Kiuchi M, Kawaoka S, et al. ( 2010) Non-molting glossy/shroud encodes a short-chain dehydrogenase/reductase that functions in the ‘Black Box' of the ecdysteroid biosynthesis pathway. Development 137: 1991–1999  Google Scholar

  37. Norum M, Tång E, Chavoshi T, Schwarz H, Linke D, Uv A, et al. ( 2010) Trafficking through COPII stabilises cell polarity and drives secretion during Drosophila epidermal differentiation. PLoS ONE 5: e10802  Google Scholar

  38. Nüsslein-Volhard C, Wieschaus E, Kluding H ( 1984) Mutations affecting the pattern of the larval cuticle in Drosophila melanogaster. I. Zygotic loci on the second chromosome. Rouxs Arch Dev Biol 193: 267–282  Google Scholar

  39. Oster II, Crang RE ( 1972) Scanning electron microscopy of Drosophila mutant and wild type eyes. Trans Amer Micros Soc 91: 600–602  Google Scholar

  40. Pai LM, Kirkpatrick C, Blanton J, Oda H, Takeichi M, Peifer M ( 1996) Drosophila α-catenin and E-cadherin bind to distinct regions of Drosophila Armadillo. J Biol Chem 271: 32411–32420  Google Scholar

  41. Peisker H, Gorb SN ( 2010) Always on the bright side of life: anti-adhesive properties of insect ommatidia grating. J Exp Biol 213: 3457–3462  Google Scholar

  42. Perry MM ( 1968) Further studies on the development of the eye of Drosophila melanogaster. I. The ommatidia. J. Morph 124: 227–248  Google Scholar

  43. Phillips AM, Smart R, Strauss R, Brembs B, Kelly LE ( 2005) The Drosophila black enigma: The molecular and behavioural characterization of the black1 mutant allele. Gene 351: 131–142  Google Scholar

  44. Richardt A, Kemme T, Wagner S, Schwarzer D, Marahiel MA, Hovemann BT ( 2003) Ebony, a novel nonribosomal peptide synthetase for β -alanine conjugation with biogenic amines in Drosophila. J Biol Chem 278: 41160–41166  Google Scholar

  45. Riedel F, Vorkel D, Eaton S ( 2011) Megalin-dependent Yellow endocytosis restricts melanization in the Drosophila cuticle. Development 138: 149–158  Google Scholar

  46. Schulze KL, Broadie K, Perin MS, Bellen HJ ( 1995) Genetic and electrophysiological studies of Drosophila syntaxin-1A demonstrate its role in nonneuronal secretion and neurotransmission. Cell 80: 311–320  Google Scholar

  47. Schwarz H, Moussian B ( 2007) Electron-microscopic and genetic dissection of arthropod cuticle differentiation. In “Modern Research and Educational Topics in Microscopy, Vol 1” Ed by A Méndez-Vilas, J Díaz, Formatex, Formatex Research Center, Badajoz, pp 316–325 Google Scholar

  48. Settle SH Jr , Green MM, Burtis KC ( 1995) The silver gene of Drosophila melanogaster encodes multiple carboxypeptidases similar to mammalian prohormone-processing enzymes. Proc Natl Acad Sci USA 92: 9470–9474  Google Scholar

  49. Stark WS, Carlson SD ( 1991) Comparison of the surfaces of glnone's ocelli and compound eyes with those of several glass alleles. DIS 70: 217–219  Google Scholar

  50. Stark WS, Carlson SD ( 2000) The glossy eye of lozenge (lz) studied by high power scanning electron microscopy (SEM) of compound eyes and ocelli. DIS 83: 49–51  Google Scholar

  51. Stark WS, Sapp R, Carlson SD ( 1989) Ultrastructure of the ocellar visual system in normal and mutant Drosophila melanogaster. J Neurogenet 5: 127–153  Google Scholar

  52. Sukontason KL, Chaiwong T, Piangjai S, Upakut S, Moophayak K, Sukontason K ( 2008) Ommatidia of blow fly, house fly, and flesh fly: implication of their vision efficiency. Parasitol Res 103: 123–131  Google Scholar

  53. Tepaß U, Knust E ( 1990) Phenotypic and developmental analysis of mutations at the crumbs locus, a gene required for the development of epithelia in Drosophila melanogaster. Roux's Arch Dev Biol 199: 189–206  Google Scholar

  54. Tepass U, Gruszynski-DeFeo E, Haag TA, Omatyar L, Török T, Hartenstein V ( 1996) shotgun encodes Drosophila E-cadherin and is preferentially required during cell rearrangement in the neurectoderm and other morphogenetically active epithelia. Genes Dev 10: 672–685  Google Scholar

  55. Tepass U, Theres C, Knust E ( 1990) crumbs encodes an EGF-like protein expressed on apical membranes of Drosophila epithelial cells and required for organization of epithelia. Cell 61: 787–799  Google Scholar

  56. Thomas HE, Stunnenberg HG, Stewart AF ( 1993) Heterodimerization of the Drosophila ecdysone receptor with retinoid X receptor and ultraspiracle. Nature 362: 471–475  Google Scholar

  57. True JR, Yeh SD, Hovemann BT, Kemme T, Meinertzhagen IA, Edwards TN, et al. ( 2005) Drosophila tan encodes a novel hydrolase required in pigmentation and vision. PLoS Genet 1: e63 Google Scholar

  58. Valcárcel R, Weber U, Jackson DB, Benes V, Ansorge W, Bohmann D, et al. ( 1999) Sec61β , a subunit of the protein translocation channel, is required during Drosophila development. J Cell Sci 112: 4389–4396  Google Scholar

  59. Woods DF, Bryant PJ ( 1993) ZO-1, DlgA and PSD-95/SAP90: homologous proteins in tight, septate and synaptic cell junctions. Mech Dev 44: 85–89  Google Scholar

  60. Yao T, Forman BM, Jiang Z, Cherbas L, Chen JD, McKeown M, et al. ( 1993) Functional ecdysone receptor is the product of EcR and Ultraspiracle genes. Nature 366: 476–479  Google Scholar


[1] Supplemental material for this article is available online.

© 2016 Zoological Society of Japan
Ryunosuke Minami, Chiaki Sato, Yumi Yamahama, Hideo Kubo, Takahiko Hariyama, and Ken-ichi Kimura "An RNAi Screen for Genes Involved in Nanoscale Protrusion Formation on Corneal Lens in Drosophila melanogaster," Zoological Science 33(6), (1 December 2016).
Received: 4 June 2016; Accepted: 1 August 2016; Published: 1 December 2016

Back to Top