Abstract
Aphids are hemimetabolous insects that undergo incomplete metamorphosis without pupation. The annual life cycle of most aphids includes both an asexual (viviparous) and a sexual (oviparous) phase. Sexual reproduction only occurs once per year and is followed by many generations of asexual reproduction, during which aphids propagate exponentially with telescopic development. Here, we discuss the potential links between viviparous embryogenesis and derived developmental features in the pea aphid Acyrthosiphon pisum, particularly focusing on germline specification and axis determination, both of which are key events of early development in insects. We also discuss potential evolutionary paths through which both viviparous and oviparous females might have come to utilize maternal germ plasm to drive germline specification. This developmental strategy, as defined by germline markers, has not been reported in other hemimetabolous insects. In viviparous females, furthermore, we discuss whether molecules that in other insects characterize germ plasm, like Vasa, also participate in posterior determination and how the anterior localization of the hunchback orthologue Ap-hb establishes the anterior-posterior axis. We propose that the linked chain of developing oocytes and embryos within each ovariole and the special morphology of early embryos might have driven the formation of evolutionary novelties in germline specification and axis determination in the viviparous aphids. Moreover, based upon the finding that the endosymbiont Buchnera aphidicola is closely associated with germ cells throughout embryogenesis, we propose presumptive roles for B. aphidicola in aphid development, discussing how it might regulate germline migration in both reproductive modes of pea aphids. In summary, we expect that this review will shed light on viviparous as well as oviparous development in aphids.
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Introduction
Aphids are small, soft-bodied, sap-sucking insects. Taxonomically, they constitute the superfamily Aphidoidea in the order Hemiptera. Developmentally, aphids are hemimetabolous: adults develop directly from nymphs without undergoing pupation or complete metamorphosis (Stern 2008). There are about 5000 named species (Blackman and Eastop 2006; Favret et al. 2016), of which at least 250 are agricultural and horticultural pests (Miller and Foottit 2017). With piercing mouthparts, aphids draw fluids from crops, resulting in plant dehydration. Additionally, aphids can serve as disease vectors, transmitting a diversity of plant viruses when moving from one plant to another while feeding (Ng and Perry 2004). Most of the extant aphid species reproduce asexually through parthenogenetic viviparity during at least part of their life cycle (Davis 2012), leading to rapid population expansions and concomitant economic damage.
The economic impact of aphids, as well as interest in the evolution of parthenogenesis, has attracted research interest for many decades. The pea aphid Acyrthosiphon pisum (Fig. 1a), as one of the first hemimetabolous species with a sequenced genome, has become a key species for studying comparative genomics across the insects. Among aphid species, A. pisum is a genomic model for exploring a range of molecular evolutionary traits for development as well as the metabolic basis of nutritional endosymbiosis (Mathers et al. 2017; The International Aphid Genomics Consortium 2010). Like many species of aphids, the pea aphid life cycle includes an asexual (viviparous) and a sexual (oviparous) phase. Thus, in one organism, it is possible to explore the unique and shared features of both developmental types. For example, there are striking spatiotemporal differences between viviparous and oviparous development. Viviparous embryogenesis is an order of magnitude faster than oviparous embryogenesis (approximately 10 days compared to 100 days; Miura et al. 2003; Shingleton et al. 2003). Viviparous eggs are also substantially smaller at the time of key patterning events in early development, with nearly a five-fold difference in egg length (Miura et al. 2003), and some key patterning differences have been described (Chung et al. 2018; Duncan et al. 2013). With the marked fecundity benefits of the asexual/viviparous mode, it is also worth noting that oviparous development is generally regarded as a seasonal feature that can be induced in the laboratory by controlling temperature and photoperiod (Ishikawa et al. 2011; Lin et al. 2014). Nevertheless, not every strain of a particular aphid species can be induced to lay eggs. Some pea aphid strains, for example, are not responsive to induction, skip oviparous development entirely, and are obligately parthenogenetic (Kanbe and Akimoto 2009). Indeed, we observe obligate parthenogenesis in the local strain of pea aphids that we handle in the laboratory (Lin and Chang 2016).
In this review, we describe what has been discovered about viviparous embryogenesis in this species. In particular, we focus on germline specification and axis determination, both of which are key developmental events during early embryogenesis. We seek to compare the differences between embryos that develop from viviparous oocytes and those that develop from oviparous oocytes. We then extend the comparison to several other established insect model organisms such as the fruit fly Drosophila melanogaster (Lynch et al. 2012), the cricket Gryllus bimaculatus (Donoughe and Extavour 2016), and the milkweed bug Oncopeltus fasciatus (Chipman 2017), all of which are exclusively sexual and oviparous.
Germline specification in the pea aphid: an exception in the Hemimetabola
Viviparous embryonic development in the pea aphid
Rapid expansion of pea aphid populations is enabled by asexual vivipary, usually during warmer months, in which unfertilized eggs undergo embryonic development within the eggs of telotrophic ovarioles, where oocytes and embryos are aligned in sequence as in an assembly line. The distinction between oocytes (stages 0–2) and embryos (stages 3–20) is determined by the appearance of the first nuclear division, which leads to the formation of the embryonic syncytium (stages 3, 4). After cellularization of the blastoderm (stages 5, 6), the maternal symbiotic bacterium Buchnera aphidicola invades the embryo through the egg posterior (stage 7). From gastrulation onward (stage 8), the posterior tip of the cellular blastoderm begins to invaginate into the interior part of the egg cavity. After that, part of the blastoderm becomes a thickened, segmented, and elongated embryo. The elongation of embryos occurs from stages 8 to 14 until just prior to the initiation of katatrepsis (embryo flip) (stage 15). Meanwhile, the remaining part of the blastoderm differentiates into the serosa, an extraembryonic membrane that enfolds the embryo. After katatrepsis, the elongated embryo retracts and the germaria become morphologically identifiable on the dorsal side. Germaria are located at the anterior end of ovarioles and contain undifferentiated cells that will form nurse cells and oocytes: in the viviparous embryos, their presence indicates that the nurse cells and the oocytes are about to differentiate. We have observed that the mature embryos (daughters; stages 16–20), in turn, already bear blastoderm stage embryos (granddaughters) (Chang et al. 2007). Hence, the 1st instar nymphs (Fig. 1a) are born pregnant. This “Russian doll” type of reproduction contributes to an exponential increase of offspring among viviparous aphid species (Stern 2008). Characteristics of developmental stages are outlined and illustrated in Fig. 1b (Miura et al. 2003).
Pea aphids possess a preformed germ plasm expressing Vas
In the asexual pea aphid, each embryo initially derives from prospective oocytes located at the posterior end of the germarium (also termed tropharium in the telotrophic-type ovariole; Büning 1985). The maturing oocytes maintain a cytoplasmic connection to, and receive nutrients from, the nurse cells of the germarium throughout oogenesis and early embryogenesis (Fig. 1b). Further investigation of how germ cells are specified will clarify how viviparous embryos originate. We studied germ-cell specification by staining embryos using an antibody against Vasa (Vas), an ATP-dependent RNA helicase that is a highly conserved germline marker in animals (Raz 2000). Immunostaining data shows that morphologically identifiable germ cells in the fully-segmented embryos are specifically labeled, indicating that the pea aphid also uses Vas as a conserved germline component (Chang et al. 2006). Through careful inspection of Vas protein localization throughout earlier developmental stages, prior to the germ cells residing in the gonads, we identified a presumptive germ plasm—a cytoplasm containing germline determinants—in the posterior region of the syncytial blastoderm (Chang et al. 2006). Together, these results strongly suggest that germline specification in the viviparous pea aphid is driven by a preformed germ plasm (Figs. 1b, 2a).
This germ plasm–driven mode, however, is not unique to viviparous reproduction in pea aphids. Vas-positive germ plasm can also be detected in the posterior region of syncytia with 32 dividing nuclei in pea aphids developing from the sexual phase of their life cycle (Lin et al. 2014). In comparison with the viviparous germ plasm, emergence of the oviparous germ plasm requires four additional rounds of nuclear division. Despite these additional nuclear divisions, in both viviparous and oviparous embryos the germ plasm is assembled during early embryogenesis while the syncytium is forming (Fig. 2a, a’) (Chang et al. 2006; Lin et al. 2014). Whether Vas that is restricted to the newly assembled germ plasm is purely maternal or partially zygotic remains uncertain. However, two pieces of evidence suggest that it is maternal Vas in the germ plasm of both viviparous and oviparous embryos: (1) expression of Vas can be continuously detected in mature oocytes as well as in newly laid eggs using both in vitro (Western blots) and in vivo (immunostaining) assays, and (2) a significant increase of Vas is not identified until the invagination of the blastoderm, suggesting that zygotic Vas is actively synthesized only from gastrulation onward (Chang et al. 2006; Lin et al. 2014).
Comparison of germline specification between pea aphids and other hemimetabolans
As determined by the presence of Vas and other germ plasm markers, the germ plasm–driven mode of germline specification in the viviparous and oviparous pea aphids is so far unique within the hemimetabolous insects (Fig. 2d). Among the established models of hemimetabolans, maternally inherited germ plasm is not detectable and germ cells are observed to be segregated from somatic cells through signal induction (Ewen-Campen et al. 2013a; Extavour and Akam 2003). For example, in the cricket Gryllus bimaculatus, germline segregation is initially detected in the abdomen following segmentation, with germline clusters appearing in abdominal segments 2 to 5 (Fig. 2b). A maternal germ plasm is not identified per se but mesodermal disruption by twist RNAi can eliminate the formation of germ cells, suggesting that germline specification in crickets depends on signals released from mesodermal cells (Ewen-Campen et al. 2013a; Mito et al. 2005). Similarly, in the grasshopper Schistocerca gregaria, an orthopteran like G. bimaculatus (Fig. 2d), germline segregation is not detected in the abdomen until it is segmented (Chang et al. 2002). In the milkweed bug Oncopeltus fasciatus, a hemipteran like aphids (Fig. 2d), germ cells initially segregated during early gastrulation can be labeled by the antisense riboprobe of Vas using whole mount in situ hybridization (WISH). However, WISH results for Vas and 18 other conserved germline genes do not mark a maternal germ plasm (Ewen-Campen et al. 2013b). Taken together, it suggests that the signal induction mode, which is a more ancestral mechanism than the germ plasm–driven mode (Extavour and Akam 2003), prevails in the hemimetabolous insects. Therefore, the germ plasm–driven mechanism identified in aphids is likely to be a derived feature.
Comparison of germline specification between pea aphids and Drosophila
In some holometabolous insects such as Drosophila, germ plasm is assembled during oogenesis (Fig. 2c, d) (Lynch et al. 2011). In the pea aphid, a hemimetabolan, assembly of the germ plasm is observed to take place later during embryogenesis (Chang et al. 2006; Lin et al. 2014). However, both Drosophila and the pea aphid share a common feature: establishment of a posteriorly localized germ plasm using maternal Vas proteins. The germ plasm forms prior to cellularization, which is termed “preformed.” This is observed regardless of whether the germ plasm is established within an oocyte or an embryo. Nevertheless, experimental results based upon ectopic expression of the pea aphid vas gene (Ap-vas1) in Drosophila suggest that formation of the maternal germ plasm in these two species arises through different molecular networks (Wang et al. 2015).
The Vas protein is a conserved germ plasm component in both Drosophila and the pea aphid, but the mechanisms by which Vas is localized are clearly different. In Drosophila, both oskar (osk) mRNA and Osk protein are molecular anchors that localize other germ plasm components, including Vas. Localization of osk/Osk to the posterior pole of oocytes initiates assembly of the germ plasm (Ephrussi et al. 1991; Ephrussi and Lehmann 1992; Kim-Ha et al. 1991). The pea aphid genome, however, does not have an orthologue of Drosophila osk (Shigenobu et al. 2010; The International Aphid Genomics Consortium 2010). This suggests that the assembly of germ plasm in the pea aphid, unlike Drosophila, is osk-independent. Ectopic expression of the pea aphid Vas (Ap-Vas1) in Drosophila oocytes, unlike the endogenous Vas (Dm-Vas), fails to localize to the germ plasm, confirming the osk-independence of Ap-Vas1 (Wang et al. 2015). Our further analysis shows that the amino acid glutamine (Gln) 527 in the conserved HELICc domain of Vas is critical to its Osk-dependent localization to the germ plasm. For example, the presence of Gln527 in Dm-Vas and the grasshopper Schistocerca Vas (Sg-Vas) facilitates successful localization of both Vas proteins to the germ plasm in Drosophila. By contrast, Ap-Vas1, Gryllus Vas, and Oncopeltus Vas, all of which lack Gln527, do not localize in the Drosophila germ plasm (Wang et al. 2015). In Schistocerca, neither an osk homolog nor a maternal germ plasm can be identified (Chang et al. 2002), but Sg-Vas with Gln527 does localize to the Osk-containing germ plasm in Drosophila, implying that this change is unrelated to the evolutionary acquisition of Osk. Whether there is a “non-Osk” molecule to anchor Ap-Vas1 to the germ plasm or Ap-Vas1 itself acts as a molecular anchor to assemble the germ plasm in pea aphids requires further investigation.
Germline migration in the pea aphid: two special features
In all insects studied to date, germ cells are specified first, then migrate (Santos and Lehmann 2004). This also applies to the pea aphid: germ cells follow a programmed migration to reach the gonadal mesoderm to form a functional gonad (Chang et al. 2007). In both asexual and sexual pea aphids, germline migration shares two characteristics that may distinguish aphids from other insects, including holometabolans. First, germ cells remain external to the embryos until katatrepsis initiates (Fig. 3). The newly formed germ cells remain outside the blastoderm after they are specified in the egg posterior (Figs. 2a, a'; 4a’–c’). Then, while the germ band is elongating, germ cells are pushed toward the egg anterior by the extending abdomen. During the embryonic inversion events of katatrepsis, the germ cells—along with the abdomen—return to the egg posterior, where the germ cells finally start to invade the interior of the embryo. After the embryonic head settles in the egg anterior, namely, the completion of katatrepsis, germ cells reside bilaterally in the dorsal region of the abdomen (Chang et al. 2009; Chang et al. 2007; Lin et al. 2014). At the same time, formation of germaria is underway (Fig. 1b, stage 16). Second, migration of the germ cells is associated with the invading endosymbionts from gastrulation onward. We have also identified the germline-endosymbiont association in the green peach aphid Myzus persicae (Chung et al. 2018), suggesting that this special phenomenon is conserved among aphid species.
In Drosophila, the primordial germ cells, or pole cells, are specified at the posterior pole of the embryos prior to blastoderm formation (Hay et al. 1988; Lasko and Ashburner 1988). When gastrulation begins, the specified germ cells are soon brought inside the embryonic cavity by their association with the invaginating posterior midgut primordium (Santos and Lehmann 2004). In contrast to Drosophila, pea aphids preserve migration of germ cells outside the embryos much longer. Results from immunostaining and WISH (Fig. 3a; Chang et al. 2007) show that germ cells remain external and are located adjacent to the extending abdomen of the viviparous embryos until the beginning of katatrepsis at stage 15 (Fig. 3a), long after the initiation of gastrulation at stage 8 of development (Miura et al. 2003). Similar locations of germ cells are also identified nearby the abdomen until early katatrepsis in the oviparous embryos (Fig. 3b; Lin et al. 2014). We suggest that these differences between aphids and flies may relate to heterochronic consequences of their modes of segmentation. In Drosophila, specification of all segments (parasegments) takes place within a short time window during cellularization of the blastoderm (Akam 1987). Because the body plan is established early, specification of the gonadal mesoderm is also determined comparatively early during late gastrulation (Boyle and DiNardo 1995; Van Doren et al. 1998). Accordingly, germline migration into the somatic gonads is known to proceed from gastrulation onward. In the pea aphid, by contrast, segmentation is not complete until the end of abdominal extension (Miura et al. 2003). Hence, the germ cells may not have a complete embryo in which to take up residence until the gonadal precursors are well-formed within the abdomen. For this reason, germ cells may be forced to remain external to the embryo in aphids until segmentation is complete just prior to katatrepsis.
At present, we can only conclude that presence of the morphologically identifiable germaria dorsal to the embryo indicates the completion of coalescence between germ cells and somatic gonads (Will 1888; Hagan 1951; Chang et al. 2007). When and where the germ cells and gonadal mesoderm first encounter each other remains uncertain, in part due to outstanding uncertainty on when bone fide germarium formation is complete. Migrating germ cells may form germ-cell clusters first and then coalesce with the gonadal mesoderm, or vice versa. Finding a specific marker to label the gonadal mesoderm, together with tracing the migrating germ cells expressing Ap-Vas1, will be helpful to understanding the formation of functional gonads in both asexual and sexual pea aphids.
With regard to the germline-endosymbiont association, we propose two potential roles of Buchnera in regulating nutrition and migration for germ cells. First, Buchnera may provide nutrients to the migrating germ cells, sustaining their development (Douglas 1998; Feng et al. 2019). Second, Buchnera may act as mediators to transmit signals released from somatic gonads, which are differentiated from the somatic mesoderm, to guide the migration of germ cells. These two roles are not mutually exclusive and Buchnera may serve both functions. If this is the case, Buchnera may spend relatively more energy on nutrient provision during early gastrulation when gonadal mesoderm has not yet formed. Later, even while transmitting guiding signals from the somatic gonads, Buchnera could still continue to provide required nutrients to the migrating germ cells.
Bacteriocytes, which are the specialized host cells that host Buchnera, may also participate in the transmission of signals for guiding germ-cell migration. In fact, it is bacteriocytes, rather than Buchnera, that directly contact the migrating germ cells in the pea aphid (Braendle et al. 2003). Guiding signals sent out from the somatic gonads may penetrate through the bacteriome—an organ-like collection of bacteriocytes—or, alternatively, the bacteriome itself might produce intermediate signals to guide the germ cells to migrate on the right path. In Drosophila, we have not found descriptions of the interaction between germ cells and bacteriocyte-like cells (Sacchi et al. 2010). However, the relationship between germline development and obligate endosymbiosis has been studied for the endosymbiont Blochmannia and their ant hosts of the hyperdiverse ant tribe Camponotini. According to Rafiqi et al. (2020), Blochmannia regulates the expression of germline genes like Vas through the Hox genes Abdominal A (abdA) and Ultrabithorax (Ubx). RNAi knockdown of abdA and Ubx results in elimination or malposition of bacteriocytes and germ cells. This suggests that the abdA/Ubx-positive bacteriocytes are involved in regulating germline development in the ants. In the seed bug Nysius plebeius and the pea aphid A. pisum, expression of abdA and Ubx can also be identified in bacteriocytes (Braendle et al. 2003; Matsuura et al. 2015), implying that the abdA/Ubx-dependent maintenance of bacteriocytes, as in ants, may be conserved and required for sustaining germline development.
Axis determination in the pea aphid: conserved and divergent aspects
Asymmetric localization: a strategy for specifying the AP axis in insects
In some insects, the embryonic anlage extends along the entire egg and all segments are determined almost simultaneously during early embryogenesis (St Johnston and Nüsslein-Volhard 1992). These “long-germ” insects usually establish the anterior-posterior (AP) axis via asymmetric localization of maternal determinants to the opposite poles of the syncytial embryos (Nüsslein -Volhard and Roth 1989; St Johnston and Nüsslein-Volhard 1992). In Drosophila, for example, anterior localization of bicoid (bcd) mRNA and posterior localization of nanos (nos) mRNA during mid-oogenesis will determine the anterior and posterior poles, respectively, of the resulting embryo (Fig. 5a) (Kugler and Lasko 2009; McGregor 2005). During mid-oogenesis, the Osk protein that is translated from the posteriorly localized osk mRNA begins recruiting germline components such as nos mRNA into the germ plasm. This posterior localization of Nos thus provides another molecular marker, in addition to bcd and osk, for marking AP polarity of the oocytes (Lasko 2012).
Although the strategy of asymmetric localization is also employed by other long-germ insects, molecular networks for specifying the AP axis appear diverse, particularly among species without a bcd orthologue. Even more strikingly, there is evidence for species using fundamentally different sets of molecules to disrupt egg symmetry and form the AP axis. For example, in the mosquito-like midge Chironomus riparius, which lacks a bcd orthologue, mRNA of the cysteine-clamp gene panish is anteriorly localized in the syncytial blastoderm (Klomp et al. 2015). RNAi of panish results in abdominal development at both embryonic poles, but ectopic expression of panish at the posterior pole does not generate a second head in the posterior. Additionally, disruption of the posteriorly localized Nos, unlike Drosophila, does not affect axial patterning. These results suggest that Chironomus utilizes a distinct pathway to generate AP polarity in which the panish protein acts as a repressor for posterior genes in the anterior and the Nos protein realizes other functions beyond its known roles for posterior patterning in Drosophila (Klomp et al. 2015). In the wasp Nasonia vitripennis, another long-germ insect lacking bcd, orthodenticle (Nv-otd1) mRNA is first localized to the oocyte posterior during early oogenesis and, then, from mid-oogenesis onward, Nv-otd1 mRNA is restricted to the oocyte anterior (Lynch et al. 2006). In addition to the posterior localization of Nv-otd1, transcripts of Nv-Nos, Nv-cad, and Nv-osk are also localized to the oocyte posterior, with all contributing to form the posterior region in Nasonia (Lynch and Desplan 2010; Lynch et al. 2011; Olesnicky et al. 2006). Together, these observations suggest that different long-germ insects make use of distinct gene regulatory connections among conserved patterning factors for directing AP patterning.
Unlike long-germ insects, the embryonic anlage of the short/intermediate germ insects—in which abdominal segments are progressively added after gastrulation—only occupies part of the egg. In the beetle Tribolium castaneum, a short/intermediate insect model, maternal Tc-germ cell-less, is known to direct the anterior localization of maternal Tc-axin (Ansari et al. 2018). After Tc-axin mRNA is maternally inherited by the fertilized egg, it promotes the zygotic expression of anterior genes such as Tc-homeobrain and Tc-zen1. Formation of the posterior region relies on Tc-cad and Wnt, both of which are operating zygotically in the growth zone. According to Ansari et al. (2018), although the initial asymmetry is formed by maternal signals, the asymmetrically localized factors for establishing the AP axis in the embryos are zygotically induced. This is different from the long-germ insects like Drosophila and Nasonia, where maternal factors specify the AP polarity and expression of zygotic genes serves to maintain the AP axis. Tribolium thus provides a useful example for interpreting how the AP axis forms in other short/intermediate germ insects including the pea aphid.
Ap-hb: a potential anterior determinant during viviparous development
In the asexual pea aphid, surprisingly, we find that the maternal hunchback (Ap-hb) mRNA is first localized to the anterior pole of stage-0 oocytes during early oogenesis (Huang et al. 2010). Anterior localization of Ap-hb can then be continuously detected in the developing oocytes and syncytial embryos prior to blastoderm formation (Figs. 4a; 5b) (Duncan et al. 2013; Huang et al. 2010). The localization pattern of Ap-hb very much resembles that of bcd in Drosophila. However, the pea aphid is missing a bcd orthologue (The International Aphid Genomics Consortium 2010). With the exception of Ap-hb, we have not found other reports of bcd-mimic localization of hb in either long- or short-germ insects (Kimelman and Martin 2012). For example, in the long-germ Drosophila, Nasonia, and Apis mellifera (honeybee), maternal hb mRNA is uniformly distributed in the oocytes and newly laid eggs (Fig. 5b) (Margolis et al. 1994; Pultz et al. 2005; Tautz et al. 1987; Wilson and Dearden 2011), and in the short-germ Schistocerca and Oncopeltus, anterior localization of the maternal hb is identified neither in the oocytes nor the uncellularized eggs (Liu and Kaufman 2004; Patel et al. 2001). Together with the finding of anterior localization of Mp-hb, an orthologue of hb in the green peach aphid, this strongly suggests that anterior localization of hb in the oocytes and early embryos is specific to the aphids (Chung et al. 2018; Huang et al. 2010). Whether this also applies to other non-aphid insects with parthenogenetic and viviparous reproduction requires further investigation.
WISH experiments using antisense riboprobes of Ap-hb in the ovaries of sexual pea aphids show that transcripts of Ap-hb are also restricted to the anterior pole of the developing oocytes. After fertilization, though, maternal Ap-hb becomes less concentrated in the egg anterior while zygotic Ap-hb is distributed along the embryonic primordium located in the egg posterior, the canonical location for formation of short-germ embryos (Figs. 4a; 5b) (Duncan et al. 2013). This suggests that (1) both asexual and sexual pea aphids utilize the anterior localization of Ap-hb to specify the anterior identity of oocytes and, perhaps, of newly laid eggs; that (2) viviparous embryos continue to employ the same mechanism to determine both the egg anterior and the embryonic anterior; but that (3) oviparous embryos, like other short-germ embryos formed in the egg posterior, do not make use of Ap-hb localization to the egg anterior (Liu and Kaufman 2005).
To date, although platforms of WISH and immunostaining have been established for detecting gene expression in the pea aphids (Chang et al. 2008; Chung et al. 2014; Lin and Chang 2016), tools for dissecting functions of genes in aphid embryos have not been successfully developed. It has therefore been difficult to uncover how Ap-hb operates for anterior determination. Nevertheless, expressions of Ap-otd and Ap-cad (Fig. 5c, d), both of which are conserved orthologues of the anterior gene otd and the posterior gene cad in insects (Lynch 2014), provide evidence to support the contribution of Ap-hb to anterior specification in viviparous embryos. First, the initial expression of Ap-otd is detected in the thickened germ band located near the egg anterior (Fig. 5c) (Huang et al. 2010), suggesting that egg anterior and embryonic anterior are formed toward the same direction. Second, Ap-cad expression detected at the opposite site of the Ap-otd expression in the germ band further verifies that the Ap-otd-positive region signifies the embryonic anterior (Fig. 5d) (Chang et al. 2013; Duncan et al. 2013). Additionally, the appearance of Ap-otd following Ap-hb localization implies that determination of the egg anterior positively regulates the formation of the embryonic anterior (Fig. 5b, c) (Huang et al. 2010). If this is the case, the process in viviparous development resembles the mode of anterior specification in long-germ insects such as Drosophila and Nasonia (Lynch et al. 2006; Riechmann and Ephrussi 2001).
Vas and Nos: potential regulators of posterior development during viviparous development
With regard to posterior development, we have not found a gene whose products are localized to the posterior pole—the pole opposite to that of Ap-hb localization—in the nascent oocytes of the viviparous pea aphid. Signals detected by cross-reacting antibodies against Vas and Nos indicate that posterior localization of these two proteins first appears in eggs undergoing nuclear division, a sign of embryogenesis initiation (Miura et al. 2003). Prominent localization of Vas and Nos has not to date been detected in the oocyte posterior (Chang et al. 2006). Expression of Ap-cad is initially identified in the newly formed germ cells and blastodermal cells in the posterior region of the blastoderm (Chang et al. 2013). These results suggest that the AP axis of both oocytes and embryos is progressively established during viviparous development. However, we cannot exclude the possibility that there is a determinant being localized synchronously with Ap-hb in the oocyte posterior. If asymmetric localization of distinct molecules is still employed to establish the AP axis in the viviparous pea aphid, it will be interesting to explore whether Vas and Nos are the determinants for posterior specification or they are the downstream targets of a posterior determinant. Their expression patterns, however, do suggest that they are likely involved in the regulation of posterior development.
Until we can successfully employ tools like RNAi or CRISPR-Cas9 to dissect gene functions in the pea aphid embryos, we cannot conclude that Vas and Nos are determinants for posterior specification. At present, the developmental roles of Ap-hb, Ap-otd, Ap-cad, Ap-vas, and Ap-nos in pea aphids can only be inferred by expression data as well as conserved roles of their orthologues in Drosophila and other insects. Additional dissection of functions of these and other developmental genes will help to clarify (1) whether specification of the anterior identity of both eggs and embryos depends on Ap-hb; (2) whether Ap-hb is an upstream regulator of Ap-otd; (3) whether Ap-vas and Ap-Nos proteins specify the posterior axes of both eggs and embryos; and (4) whether Ap-cad is a downstream target of the products encoded by the Ap-vas and Ap-nos genes. Transcriptome analysis of the posterior genes in the pea aphid, including conserved and novel, should also provide more candidates for functional examination.
Germline expression of Ap-hb/Ap-Hb in the viviparous pea aphid
Functional analysis of developmental genes in the pea aphid, if successfully developed, will provide answers to another question: how does Ap-hb regulate germline development? This question is prompted by the finding that Ap-hb mRNA and protein, in addition to their conserved expression in the neural system, are identified in the germ cells throughout embryogenesis in the viviparous pea aphid (Fig. 4) (Chung et al. 2018). Germline expression of Mp-hb can also be detected in viviparous green peach aphids, but a germline role for hb has not been reported outside Aphidoidea. Whether Ap-hb and Mp-hb are expressed in the germline of oviparous embryos remains unknown. The available evidence suggests that germline expression of hb, like anterior localization of hb, is a derived characteristic among the viviparous aphids. The absence of Ap-hb and Ap-Hb in the preformed germ plasm implies that the Ap-hb gene is not involved in germline specification (Chung et al. 2018; Huang et al. 2010). We note that germline expression of Ap-hb/Ap-Hb is detected soon after the blastoderm is formed, during which anterior localization of the maternal Ap-hb is missing (Figs. 4a, a'; 5b) (Chung et al. 2018). This suggests that germline expression of Ap-hb is zygotic. Additionally, if germline Ap-hb mRNA is synthesized for anterior localization of the oocytes in the embryonic gonads, germ cells—precursors of the oocytes—could already begin producing Ap-hb once they are settled within the germaria after katatrepsis. Early initiation of germline expression of Ap-hb, when germ cells are newly formed, also implies that Ap-hb may participate in the maintenance of germline development during embryogenesis.
Conclusion and evolutionary aspects
In this review, we have discussed germline specification and axis determination in the pea aphids, focusing in particular on the asexual and viviparous morphs. Embryos of asexual pea aphids have an extending abdomen before katatrepsis and are therefore categorized as short-germ embryos, whose abdominal segments are gradually established during mid-embryogenesis (stages 7 to 14). Prior to abdominal extension (stages 3 to 6), however, the blastoderm occupies most of the egg. In this feature, aphid embryogenesis is more similar to that of long-germ embryos, whose blastoderm length is almost equivalent to the egg length. This “long germ-like” feature is not observed in other studied short-germ insects such as grasshoppers and crickets, whose embryonic primordia only occupy a small proportion of the egg posterior (Donoughe and Extavour 2016; Patel et al. 2001; Schröder et al. 2008).
In combining characteristics typical of development in both short- and long-germ embryos, viviparous development in the pea aphid exhibits three noteworthy features of early development. First, germline specification is driven by a preformed germ plasm expressing the conserved germline marker Vas (Chang et al. 2006). This is so far the sole example identified among hemimetabolans of Vas being employed as a component of the preformed germ plasm. Second, specification of the anterior identity of oocytes and embryos takes place in the same region and toward the same direction. The oocyte anterior is characterized by Ap-hb localization and the embryo anterior by Ap-otd expression (Huang et al. 2010). This differs from other studied short-germ insects, including the sexual pea aphids (Duncan et al. 2013; Lin et al. 2014), whose progeny develops oviparously and whose embryonic primordia arise from a small proportion in the egg posterior. Third, the mRNA of hb and its translated protein are expressed in the germ cells throughout embryogenesis (Chung et al. 2018). Expression of hb in the neural system during development is a highly conserved feature among insects, yet to date, germline expression of hb has only been identified in embryos of asexual aphids.
Identification of a Vas-positive germ plasm in oviparous oocytes of sexual pea aphid, such as the germline expression of Ap-hb mentioned above, is unexpected (Lin et al. 2014). These results suggest that sexual pea aphids, like other sexually reproduced hemimetabolans, might specify germ cells with the more ancestral approach, termed the signal-induction mode (Extavour and Akam 2003). After asexual vivipary evolved, the germ plasm–driven mode then co-evolved for development within the viviparous morphs and was eventually also utilized for development during oviparous reproduction. Afterwards, it was inherited by the oviparous morphs. However, we cannot exclude the possibility that germ plasm–driven development evolved simultaneously in viviparous and oviparous reproduction in aphids.
With regard to the anterior localization of hb, we hypothesize that it might be a feature that evolved in response to the invading endosymbiont Buchnera. Allowing precise invasion of endosymbionts in the embryo posterior from gastrulation onward requires setting the orientations of the eggs and embryos before the endosymbionts can invade: localization of hb transcripts may be utilized to label the egg and embryo anterior for this purpose. Likewise, posterior localization of Vas/Nos may fulfill the same purpose through a strategy of asymmetric localization.
In summary, we propose that the parthenogenic viviparity, an evolutionary novelty, drove the evolution of observed developmental novelties in germline specification and AP axis determination in the viviparous pea aphid. Whether establishment of the dorsal-ventral (DV) axis also exhibits asymmetric localization requires further investigation. To dissect developmental mechanisms in depth, the making of transgenic aphids and the development of effective approaches for dissecting gene functions are crucial. As more unique features of aphid development are uncovered, we believe they will serve the foundation for inventing more aphid-specific strategies to suppress the expansion of aphids.
Data availability
All data is provided in the text and the figures.
References
Akam M (1987) The molecular basis for metameric pattern in the Drosophila embryo. Development 101(1):1–22. https://doi.org/10.1242/dev.101.1.1
Ansari S, Troelenberg N, Dao VA, Richter T, Bucher G, Klingler M (2018) Double abdomen in a short-germ insect: zygotic control of axis formation revealed in the beetle Tribolium castaneum. Proc Natl Acad Sci USA 115(8):1819–1824. https://doi.org/10.1073/pnas.1716512115
BDGP (2021) http://insitu.fruitfly.org. Accessed 10 Dec 2021
Blackman RL (1978) Early development of parthenogenetic egg in 3 species of aphids (Homoptera: Aphididae). Int J Insect Morphol 7(1):33–44. https://doi.org/10.1016/S0020-7322(78)80013-0
Blackman RL, Eastop VF (2006) Aphids on the world’s herbaceous plants and shrubs. Volume 1: host lists and keys. Volume 2: the aphids. John Wiley & Sons Ltd, Chichester, in conjunction with The Natural History Museum, London, Chichester and London
Boyle M, DiNardo S (1995) Specification, migration and assembly of the somatic cells of the Drosophila gonad. Development 121(6):1815–1825. https://doi.org/10.1242/dev.121.6.1815
Braendle C, Miura T, Bickel R, Shingleton AW, Kambhampati S, Stern DL (2003) Developmental origin and evolution of bacteriocytes in the aphid-Buchnera symbiosis. PLoS Biol 1(1):E21. https://doi.org/10.1371/journal.pbio.0000021
Büning J (1985) Morphology, ultrastructure, and germ cell cluster formation in ovarioles of aphids. J Morphol 186(2):209–221. https://doi.org/10.1002/jmor.1051860206
Chang C-c, Dearden P, Akam M (2002) Germ line development in the grasshopper Schistocerca gregaria: vasa as a marker. Dev Biol 252(1):100–118. https://doi.org/10.1006/Dbio.2002.0840
Chang C-c, Lee WC, Cook CE, Lin GW, Chang T (2006) Germ-plasm specification and germline development in the parthenogenetic pea aphid Acyrthosiphon pisum: Vasa and Nanos as markers. Int J Dev Biol 50(4):413–421. https://doi.org/10.1387/ijdb.052100cc
Chang C-c, Lin GW, Cook CE, Horng SB, Lee HJ, Huang TY (2007) Apvasa marks germ-cell migration in the parthenogenetic pea aphid Acyrthosiphon pisum (Hemiptera: Aphidoidea). Dev Genes Evol 217(4):275–287. https://doi.org/10.1007/s00427-007-0142-7
Chang C-c, Huang TY, Shih CL, Lin GW, Chang TP, Chiu H, Chang WC (2008) Whole-mount identification of gene transcripts in aphids: protocols and evaluation of probe accessibility. Arch Insect Biochem Physiol 68(4):186–196. https://doi.org/10.1002/Arch.20243
Chang C-c, Huang TY, Cook CE, Lin GW, Shih CL, Chen RPY (2009) Developmental expression of Apnanos during oogenesis and embryogenesis in the parthenogenetic pea aphid Acyrthosiphon pisum. Int J Dev Biol 53(1):169–176. https://doi.org/10.1387/ijdb.082570cc
Chang C-c, Hsiao YM, Huang TY, Cook CE, Shigenobu S, Chang TH (2013) Noncanonical expression of caudal during early embryogenesis in the pea aphid Acyrthosiphon pisum: maternal cad-driven posterior development is not conserved. Insect Mol Biol 22(4):442–455. https://doi.org/10.1111/imb.12035
Chipman AD (2017) Oncopeltus fasciatus as an evo-devo research organism. Genesis 55:e23020. https://doi.org/10.1002/dvg.23020
Chung C-y, Cook CE, Lin GW, Huang TY, Chang C-c (2014) Reliable protocols for whole-mount fluorescent in situ hybridization (FISH) in the pea aphid Acyrthosiphon pisum: a comprehensive survey and analysis. Insect Sci 21(3):265–277. https://doi.org/10.1111/1744-7917.12086
Chung C-y, Hsiao YM, Huang TY, Chang TH, Chang C-c (2018) Germline expression of the hunchback orthologues in the asexual viviparous aphids: a conserved feature within the Aphididae. Insect Mol Biol 27(6):752–765. https://doi.org/10.1111/imb.12514
Davis GK (2012) Cyclical parthenogenesis and viviparity in aphids as evolutionary novelties. J Exp Zool B Mol Dev Evol 318(6):448–459. https://doi.org/10.1002/jez.b.22441
Donoughe S, Extavour CG (2016) Embryonic development of the cricket Gryllus bimaculatus. Dev Biol 411(1):140–156. https://doi.org/10.1016/j.ydbio.2015.04.009
Douglas AE (1998) Nutritional interactions in insect-microbial symbioses: aphids and their symbiotic bacteria Buchnera. Annu Rev Entomol 43:17–37. https://doi.org/10.1146/annurev.ento.43.1.17
Duncan EJ, Leask MP, Dearden PK (2013) The pea aphid (Acyrthosiphon pisum) genome encodes two divergent early developmental programs. Dev Biol 377(1):262–274. https://doi.org/10.1016/j.ydbio.2013.01.036
Ephrussi A, Lehmann R (1992) Induction of germ cell formation by oskar. Nature 358(6385):387–392. https://doi.org/10.1038/358387a0
Ephrussi A, Dickinson LK, Lehmann R (1991) Oskar organizes the germ plasm and directs localization of the posterior determinant nanos. Cell 66(1):37–50. https://doi.org/10.1016/0092-8674(91)90137-n
Ewen-Campen B, Donoughe S, Clarke DN, Extavour CG (2013a) Germ cell specification requires zygotic mechanisms rather than germ plasm in a basally branching insect. Curr Biol 23(10):835–842. https://doi.org/10.1016/j.cub.2013.03.063
Ewen-Campen B, Jones TE, Extavour CG (2013b) Evidence against a germ plasm in the milkweed bug Oncopeltus fasciatus, a hemimetabolous insect. Biol Open 2(6):556–568. https://doi.org/10.1242/bio.20134390
Extavour CG, Akam M (2003) Mechanisms of germ cell specification across the metazoans: epigenesis and preformation. Development 130(24):5869–5884. https://doi.org/10.1242/dev.00804
Favret C, Blackman RL, Miller GL, Victor B (2016) Catalog of the phylloxerids of the world (Hemiptera, Phylloxeridae). Zookeys 629:83–101. https://doi.org/10.3897/zookeys.629.10709
Feng H, Edwards N, Anderson CMH, Althaus M, Duncan RP, Hsu YC, Luetje CW, Price DRG, Wilson ACC, Thwaites DT (2019) Trading amino acids at the aphid-Buchnera symbiotic interface. Proc Natl Acad Sci USA 116(32):16003–16011. https://doi.org/10.1073/pnas.1906223116
Gao Q, Wang Y, Finkelstein R (1996) Orthodenticle regulation during embryonic head development in Drosophila. Mech Dev 56:3–15. https://doi.org/10.1016/0925-4773(96)00504-7
Hagan HR (1951) Embryology of the viviparous insects. Part II: Embryogenesis. Ronald Press, New York, pp 356–392
Hay B, Jan LY, Jan YN (1988) A protein component of Drosophila polar granules is encoded by vasa and has extensive sequence similarity to ATP-dependent helicases. Cell 55(4):577–587. https://doi.org/10.1016/0092-8674(88)90216-4
Huang TY, Cook CE, Davis GK, Shigenobu S, Chen RP, Chang C-c (2010) Anterior development in the parthenogenetic and viviparous form of the pea aphid, Acyrthosiphon pisum: hunchback and orthodenticle expression. Insect Mol Biol 19(Suppl 2):75–85. https://doi.org/10.1111/j.1365-2583.2009.00940.x
Ishikawa A, Ogawa K, Gotoh H, Walsh TK, Tagu D, Brisson JA, Rispe C, Jaubert-Possamai S, Kanbe T, Tsubota T et al (2011) Juvenile hormone titre and related gene expression during the change of reproductive modes in the pea aphid. Insect Mol Biol 21(1):49–60. https://doi.org/10.1111/j.1365-2583.2011.01111.x
Kanbe T, Akimoto S (2009) Allelic and genotypic diversity in long-term asexual populations of the pea aphid, Acyrthosiphon pisum in comparison with sexual populations. Mol Ecol 18(5):801–816. https://doi.org/10.1111/j.1365-294X.2008.04077.x
Kimelman D, Martin BL (2012) Anterior-posterior patterning in early development: three strategies. Wiley Interdiscip Rev Dev Biol 1(2):253–266. https://doi.org/10.1002/wdev.25
Kim-Ha J, Smith JL, Macdonald PM (1991) oskar mRNA is localized to the posterior pole of the Drosophila oocyte. Cell 66(1):23–35. https://doi.org/10.1016/0092-8674(91)90136-m
Klomp J, Athy D, Kwan CW, Bloch NI, Sandmann T, Lemke S, Schmidt-Ott U (2015) Embryo development. A cysteine-clamp gene drives embryo polarity in the midge Chironomus. Science 348(6238):1040–1042. https://doi.org/10.1126/science.aaa7105
Kugler JM, Lasko P (2009) Localization, anchoring and translational control of oskar, gurken, bicoid and nanos mRNA during Drosophila oogenesis. Fly 3(1):15–28. https://doi.org/10.4161/fly.3.1.7751
Lasko P (2012) mRNA localization and translational control in Drosophila oogenesis. Cold Spring Harb Perspect Biol 4(10):a012294. https://doi.org/10.1101/cshperspect.a012294
Lasko PF, Ashburner M (1988) The product of the Drosophila gene vasa is very similar to eukaryotic initiation factor-4A. Nature 335(6191):611–617. https://doi.org/10.1038/335611a0
Lin GW, Chang C-c (2016) Identification of critical conditions for immunostaining in the pea aphid embryos: increasing tissue permeability and decreasing background staining. JoVE 108:e53883. https://doi.org/10.3791/53883
Lin GW, Cook CE, Miura T, Chang C-c (2014) Posterior localization of ApVas1 positions the preformed germ plasm in the sexual oviparous pea aphid Acyrthosiphon pisum. EvoDevo 5:18. https://doi.org/10.1186/2041-9139-5-18
Liu PZ, Kaufman TC (2004) hunchback is required for suppression of abdominal identity, and for proper germband growth and segmentation in the intermediate germband insect Oncopeltus fasciatus. Development 131(7):1515–1527. https://doi.org/10.1242/dev.01046
Liu PZ, Kaufman TC (2005) Short and long germ segmentation: unanswered questions in the evolution of a developmental mode. Evol Dev 7(6):629–646. https://doi.org/10.1111/j.1525-142X.2005.05066.x
Lynch JA (2014) Diversity of molecules and mechanisms in establishing insect anterior-posterior polarity. Curr Opin Insect Sci 1:39–44. https://doi.org/10.1016/j.cois.2014.05.003
Lynch JA, Desplan C (2010) Novel modes of localization and function of nanos in the wasp Nasonia. Development 137(22):3813–3821. https://doi.org/10.1242/dev.054213
Lynch JA, Brent AE, Leaf DS, Pultz MA, Desplan C (2006) Localized maternal orthodenticle patterns anterior and posterior in the long germ wasp Nasonia. Nature 439(7077):728–732. https://doi.org/10.1038/nature04445
Lynch JA, Ozuak O, Khila A, Abouheif E, Desplan C, Roth S (2011) The phylogenetic origin of oskar coincided with the origin of maternally provisioned germ plasm and pole cells at the base of the Holometabola. PLoS Genet 7(4):e1002029. https://doi.org/10.1371/journal.pgen.1002029
Lynch JA, El-Sherif E, Brown SJ (2012) Comparisons of the embryonic development of Drosophila, Nasonia, and Tribolium. WIREs Dev Biol 1:16–39. https://doi.org/10.1002/wdev.3
Margolis JS, Borowsky M, Shim CW, Posakony JW (1994) A small region surrounding the distal promoter of the hunchback gene directs maternal expression. Dev Biol 163(2):381–388. https://doi.org/10.1006/dbio.1994.1156
Mathers TC, Chen Y, Kaithakottil G, Legeai F, Mugford ST, Baa-Puyoulet P, Bretaudeau A, Clavijo B, Colella S, Collin O et al (2017) Rapid transcriptional plasticity of duplicated gene clusters enables a clonally reproducing aphid to colonise diverse plant species. Genome Biol 18(1):27. https://doi.org/10.1186/s13059-016-1145-3
Matsuura Y, Kikuchi Y, Miura T, Fukatsu T (2015) Ultrabithorax is essential for bacteriocyte development. Proc Natl Acad Sci USA 112(30):9376–9381. https://doi.org/10.1073/pnas.1503371112
McGregor AP (2005) How to get ahead: the origin, evolution and function of bicoid. Bioessays 27(9):904–913. https://doi.org/10.1002/bies.20285
Miller GL, Foottit RG (2017) The taxonomy of crop pests: the aphids. In insect biodiversity. John Wiley & Sons, Ltd, Hoboken, NJ, USA
Misof B, Liu S, Meusemann K, Peters RS, Donath A, Mayer C, Frandsen PB, Ware J, Flouri T, Beutel RG et al (2014) Phylogenomics resolves the timing and pattern of insect evolution. Science 346(6210):763–767. https://doi.org/10.1126/science.1257570
Mito T, Sarashina I, Zhang H, Iwahashi A, Okamoto H, Miyawaki K, Shinmyo Y, Ohuchi H, Noji S (2005) Non-canonical functions of hunchback in segment patterning of the intermediate germ cricket Gryllus bimaculatus. Development 132(9):2069–2079. https://doi.org/10.1242/dev.01784
Miura T, Braendle C, Shingleton A, Sisk G, Kambhampati S, Stern DL (2003) A comparison of parthenogenetic and sexual embryogenesis of the pea aphid Acyrthosiphon pisum (Hemiptera: Aphidoidea). J Exp Zool (Mol Dev Evol) 295(1):59–81. https://doi.org/10.1002/jez.b.3
Mlodzik M, Gehring WJ (1987) Expression of the caudal gene in the germ line of Drosophila: formation of an RNA and protein gradient during early embryogenesis. Cell 48:465–478. https://doi.org/10.1016/0092-8674(87)90197-8
Ng JCK, Perry KL (2004) Transmission of plant viruses by aphid vectors. Mol Plant Pathol 5(5):505–511. https://doi.org/10.1111/j.1364-3703.2004.00240.x
Nüsslein -Volhard C, Roth S (1989) Axis determination in insect embryos. Ciba Found Symp 144:37-55; discussion 55-64, 92-98. 10.1002/9780470513798.ch4
Olesnicky EC, Brent AE, Tonnes L, Walker M, Pultz MA, Leaf D, Desplan C (2006) A caudal mRNA gradient controls posterior development in the wasp Nasonia. Development 133(20):3973–3982. https://doi.org/10.1242/dev.02576
Patel NH, Hayward DC, Lall S, Pirkl NR, DiPietro D, Ball EE (2001) Grasshopper hunchback expression reveals conserved and novel aspects of axis formation and segmentation. Development 128(18):3459–3472. https://doi.org/10.1242/dev.128.18.3459
Pultz MA, Westendorf L, Gale SD, Hawkins K, Lynch J, Pitt JN, Reeves NL, Yao JC, Small S, Desplan C et al (2005) A major role for zygotic hunchback in patterning the Nasonia embryo. Development 132(16):3705–3715. https://doi.org/10.1242/dev.01939
Rafiqi AM, Rajakumar A, Abouheif E (2020) Origin and elaboration of a major evolutionary transition in individuality. Nature 585(7824):239–244. https://doi.org/10.1038/s41586-020-2653-6
Raz E (2000) The function and regulation of vasa-like genes in germ-cell development. Genome Biol 1 (3):reviews1017.1011-1017.1016. https://doi.org/10.1186/gb-2000-1-3-reviews1017
Riechmann V, Ephrussi A (2001) Axis formation during Drosophila oogenesis. Curr Opin Genet Dev 11(4):374–383. https://doi.org/10.1016/S0959-437X(00)00207-0
Sacchi L, Genchi M, Clementi E, Negri I, Alma A, Ohler S, Sassera D, Bourtzis K, Bandi C (2010) Bacteriocyte-like cells harbour Wolbachia in the ovary of Drosophila melanogaster (Insecta, Diptera) and Zyginidia pullula (Insecta, Hemiptera). Tissue Cell 42(5):328–333. https://doi.org/10.1016/j.tice.2010.07.009
Santos AC, Lehmann R (2004) Germ cell specification and migration in Drosophila and beyond. Curr Biol 14(14):R578–R589. https://doi.org/10.1016/j.cub.2004.07.018
Schröder R, Beermann A, Wittkopp N, Lutz R (2008) From development to biodiversity—Tribolium castaneum, an insect model organism for short germband development. Dev Genes Evol 218(3-4):119–126. https://doi.org/10.1007/s00427-008-0214-3
Shigenobu S, Bickel RD, Brisson JA, Butts T, Chang C-c, Christiaens O, Davis GK, Duncan EJ, Ferrier DEK, Iga M et al (2010) Comprehensive survey of developmental genes in the pea aphid, Acyrthosiphon pisum: frequent lineage-specific duplications and losses of developmental genes. Insect Mol Biol 19:47–62. https://doi.org/10.1111/j.1365-2583.2009.00944.x
Shingleton AW, Sisk GC, Stern DL (2003) Diapause in the pea aphid (Acyrthosiphon pisum) is a slowing but not a cessation of development. BMC Dev Biol 3:7. https://doi.org/10.1186/1471-213X-3-7
St Johnston D, Nüsslein-Volhard C (1992) The origin of pattern and polarity in the Drosophila embryo. Cell 68(2):201–219. https://doi.org/10.1016/0092-8674(92)90466-P
Stern DL (2008) Aphids. Curr Biol 18:504–505. https://doi.org/10.1016/j.cub.2008.03.034
Tautz D, Lehmann R, Schnürch H, Schuh R, Seifert E, Kienlin A, Jones K, Jäckle H (1987) Finger protein of novel structure encoded by hunchback, a second member of the gap class of Drosophila segmentation genes. Nature 327(6121):383–389. https://doi.org/10.1038/327383a0
The International Aphid Genomics Consortium (2010) Genome sequence of the pea aphid Acyrthosiphon pisum. PLoS Biol 8(2):e1000313. https://doi.org/10.1371/journal.pbio.1000313
Van Doren M, Broihier HT, Moore LA, Lehmann R (1998) HMG-CoA reductase guides migrating primordial germ cells. Nature 396(6710):466–469. https://doi.org/10.1038/24871
Wang SC, Hsu HJ, Lin GW, Wang TF, Chang C-c, Lin MD (2015) Germ plasm localisation of the HELICc of Vasa in Drosophila: analysis of domain sufficiency and amino acids critical for localisation. Sci Rep 5:14703. https://doi.org/10.1038/srep14703
Will L (1888) Entwicklungsgeschichte der viviparen Aphiden. Zool Jahrb (Anat) 3:201–286
Wilson MJ, Dearden PK (2011) Diversity in insect axis formation: two orthodenticle genes and hunchback act in anterior patterning and influence dorsoventral organization in the honeybee (Apis mellifera). Development 138(16):3497–3507. https://doi.org/10.1242/dev.067926
Acknowledgements
We thank former laboratory members that contributed to the establishment of platforms for studying aphid development at the National Taiwan University (NTU). In addition, we are grateful to the Technology Commons in the College of Life Science NTU for technical support on confocal microscopy. We thank Tien-Hsien Chang, Shuji Shigenobu, and Toru Miura for kind collaboration in the past decade. Finally, we thank three anonymous reviewers and the editor for their extremely dedicated revision efforts and insightful remarks, all of which improved the manuscript significantly.
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This work was supported by the Ministry of Science and Technology (110-2811-B-002-548 for CYC and CC; 109-2313-B-002-043-MY3 and 106-2313-B-002-018-MY3 for CYC, MDL, and CC) and the NTU (G049961 for CC, GWL, and other authors).
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Lin, GW., Chung, Cy., Cook, C.E. et al. Germline specification and axis determination in viviparous and oviparous pea aphids: conserved and divergent features. Dev Genes Evol 232, 51–65 (2022). https://doi.org/10.1007/s00427-022-00690-7
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DOI: https://doi.org/10.1007/s00427-022-00690-7