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Volume 17, Number 13, Issue of July 1, 1997 pp. 5108-5118
Copyright ©1997 Society for Neuroscience

Diverse Expression and Distribution of Shaker Potassium Channels during the Development of the Drosophila Nervous System

Oscar Rogero, Barbara Hämmerle, and Francisco J. Tejedor

Instituto de Neurociencias, Instituto Cajal, Consejo Superior de Investigaciones Cientificas, Universidad de Alicante, San Juan, 03080 Alicante, Spain

ABSTRACT
INTRODUCTION
MATERIALS AND METHODS
RESULTS
DISCUSSION
FOOTNOTES
REFERENCES

ABSTRACT

The spatio-temporal expression of Shaker (Sh) potassium channels (Kch) in the developing and adult nervous system of Drosophila has been studied at the molecular and histological level using specific antisera. Sh Kch are distributed in most regions of the nervous system, but their expression is restricted to only certain populations of cells. Sh Kch have been found in the following three locations: in synaptic areas of neuropile, in axonal fiber tracks, and in a small number of neuronal cell bodies. This wide subcellular localization, together with a diverse distribution, implicates Sh Kch in multiple neuronal functions.

Experiments performed with Sh mutants that specifically eliminate a few of the Sh Kch splice variants clearly demonstrate an abundant differential expression and usage of the wide repertoire of Sh isoforms, but they do not support the idea of extensive segregation of these isoforms among different populations of neurons. Sh Kch are predominantly expressed at late stages of postembryonic development and adulthood. Strikingly, wide changes in the repertoire of Sh splice isoforms occur some time after the architecture of the nervous system is complete, indicating that the expression of Sh Kch contributes to the final refinements of neuronal differentiation. These late changes in the expression and distribution of Sh Kch seem to correlate with activity patterns suggesting that Sh Kch may be involved in adaptative mechanisms of excitability.

Key words: potassium channels; Shaker; Drosophila; K-channel expression; K-channel localization; K-channel distribution

INTRODUCTION

In the last decade, the combination of electrophysiology and molecular biology has yielded great advances in the understanding of the molecular diversity and the structure-function relationship of ionic channels (Hille, 1992). In spite of this, the specific function of each particular channel transcript is not well understood. This is often because of the lack of correlation between in vitro-expressed cloned channels and in vivo functions.

Potassium channels (Kch) are probably the most diverse class among ion channels (Rudy, 1988; Miller, 1991; Rudy et al., 1991; Jan and Jan, 1992, 1994; Pongs, 1992; Salkoff et al., 1992). Multiple Kch proteins, having a common central region and different N and C termini, are produced from the Shaker (Sh) transcription unit by differential and alternative splicing (Kamb et al., 1988; Pongs et al., 1988; Schwarz et al., 1988). Four Sh subunits assemble to form a functional channel (MacKinnon, 1991) with different electrical properties depending on the subunit composition (Iverson and Rudy, 1990; Stocker M et al., 1990). Thus, the regulation of both transcription and splicing of Sh may determine the intrinsic electrical properties of Drosophila neurons.

The study of channels in the nervous system has usually relied on electrical recording from cell bodies. Unfortunately, this is difficult to apply to the study of channels located in dendrites, axons, synapses, and so forth. In addition, very little is known about the mechanism of subcellular distribution and the subunit association of channel proteins. An understanding of the role played by the broad repertoire of ion channels expressed in the nervous system, therefore, would require the study of channel distribution in nerve cell populations and their subcellular localization within the complex neuronal architecture. Immunohistological techniques, using high-affinity antibodies against specific ion channels, provide the most convenient method for approaching this question. The possibility of carrying this immunocytological study to Drosophila presents the additional advantage of using the numerous existing mutations to genetically dissect regulatory pathways.

Surprisingly, there have been only two reports in the literature on the immunolocalization of K+-channels in Drosophila (Schwarz et al., 1990; Becker et al., 1995). The shortage of experimental results in such an active field of research probably reflects the lack of high-affinity antisera for elucidating this important matter.

We have recently raised an antiserum against Sh Kch that specifically labels multiple Sh proteins in extracts of nervous tissue at different developmental stages (Rogero and Tejedor, 1995).

As an additional step toward unraveling the roles played by this family of ion channels, the present study is the first to examine the tissular distribution and cellular localization of Sh Kch during the development of the nervous system of Drosophila. Thus, the aim of this work is to understand how the wide repertoire of Kch subunit variants generated by the Sh transcription unit is spatially and temporally expressed.

MATERIALS AND METHODS

Fly stocks, culture, and harvesting. Drosophila melanogaster stocks were grown in standard medium at 25°C with 12 hr dark/light cycles. The Canton-S (CS) strain was used as a wild-type (wt) control, although no differences were found with other common wt strains such as Berlin. w Mutants, which lack eye pigment, were used as wt control flies for most experiments examining expression in the retina. Males of the mutant strains B55D/W32P/C(1)M3/0 (Df); T(X;Y)W32/FM7a/Y (W32); T(X,Y)B55/y w f XX (B55); ShE62/C(1)M3; w sev; and sc10.1 were also used. Staging of pupae was according to Bainbridge and Bownes (1981).

Antisera production and purification. Production and affinity purification of the antiserum alpha -ShHX1 was performed as reported previously (Rogero and Tejedor, 1995). In brief, rabbit antiserum was raised against a recombinant fusion protein containing a sequence stretch of the central core region that is common to all Sh splice variants. Antisera were affinity-purified and their specificity tested by comparing Western blot (WB) analysis of total proteins from CS and Sh-deficient (Df) flies, which lack genomic DNA from the Sh coding region (Pongs et al., 1988). The lack of any labeled band in the Df immunoblot clearly demonstrates the high specificity of these antisera (Rogero and Tejedor, 1995).

Electrophoresis, WB, and immunoblots. Regular monodimensional SDS-PAGE was used according to Laemmli (1970) and modified by Rogero and Tejedor (1995). Tissue samples (whole flies, pupae, and so forth) were homogenized at 80°C in 50 mM Tris, 25 mM KCl, 2 mM EDTA, 0.3 M sucrose, and 2% SDS, pH 7.4, with a microglass potter. Samples were then boiled for 5 min in SDS-PAGE sample buffer and 20 mM DTT. Gels were usually loaded with 12 µl of each sample. WB were done by electrotransferring the proteins of the gel to nitrocellulose membranes under standard conditions. Immunoblots were performed as described previously (Rogero and Tejedor, 1995). The chemiluminescent ECL (Amersham, Arlington Heights, IL) method was used for the final detection of antibody-binding.

Histology and immunohistology. Mature third instar larvae were dissected in cold Ringer's solution, and brains were fixed at 0°C in nonalcoholic Bouin's fixative for 30-60 min. After immunostaining, brains were dehydrated with alcohol and embedded in SPURR for microsectioning.

Ether-anesthetized flies with no previous fixation were rapidly embedded in Tissue-Tek (Miles, Elkhart, IN), appropriately oriented, and frozen instantaneously in liquid nitrogen. Frontal, horizontal, and sagittal 12 µM sections were made in a microtome cryostat and fixed in nonalcoholic Bouins at 4-8°C for 1 hr. Tangential cryostat sections from retina were sequentially fixed with paraformaldehyde (10 min) and nonalcoholic Bouin's fixative (30 min) at 4-8°C.

Immunostaining of whole-mount and cryostat sections was performed with an overnight incubation at 8-10°C with affinity-purified alpha -ShHX1 antiserum (Rogero and Tejedor, 1995). A biotin-coupled anti-rabbit IgG and an avidin-biotin-HRP complex were used sequentially under standard conditions to produce the final reaction of DAB.

To see the cellular structure of the retina, proboscides and air sacks were quickly removed from heads in ice-cold 4% paraformaldehyde. Heads were sequentially fixed with paraformaldehyde and Bouin's fixative as before, and embedded in SPURR. Tangential 4 µM sections were made of the retina and stained with 0.02 methylene blue/0.02% toluidine blue in 0.1% borax.

Toluidine blue counterstaining of either plastic or cryostat sections was performed at 40°C with 0.05% toluidine blue in 0.1% borax. Under these conditions, only cellular structures lacking DAB-precipitate are stained blue.

RESULTS

Distribution and localization of Sh Kch in the CNS

In a previous immunochemical study (Rogero and Tejedor, 1995), we found Sh Kch to be expressed throughout development. The following two waves of expression were detected by WB: a small larval peak and a long second wave that began at the late pupal stage and reached a plateau in the adult. Accordingly, our immunohistological study starts with the third instar larval CNS. As shown in Figure 1A, the alpha -ShHX1 antiserum labels the neuropile over the entire whole-mount larval brain. The absence of labeling in the nervous system of Df flies (Fig. 1B) demonstrates the high specificity of this antiserum. The staining is particularly intense in the mushroom bodies (MB), which can be recognized easily by their characteristic morphology (Fig. 1A,C,D). Besides this wide and intense neuropile labeling, a small number of immunostained somata were detected at different focal planes throughout the larval brain. This includes a well-defined distribution pattern of neurons (Fig. 1D, blue spots) such as those located in a medial plane close to the MB (Fig. 1A,C) as well as a few neuroblasts (Fig. 1D, red spots) that appear in thoracic and abdominal proliferative regions with a nonrepetitive pattern. Unfortunately, we have been unable to identify these cells, because their distribution pattern does not fit well with any map of neuronal families expressing particular neurochemical properties such as neurotransmitters and neuropeptides, or a given molecular marker (Buchner et al., 1986; White et al., 1986; Budnik and White, 1988; Vallés and White, 1988; Lundell and Hirsh, 1994).
Fig. 1. Immunolocalization of Sh Kch in third instar larval brains. A, Immunostained brain from mature third instar CS larvae. Small arrows point to labeled somata. B, Parallel control of a Df brain. Photographs were taken at 200× magnification from a ventral view. C, Higher magnification (400×) of the boxed area in A, showing immunolabeling of MB neuropile and a few cell bodies (arrows) at a medial focal plane. D, Schematic representation of the ventral-dorsal projection of a larval brain immunostained with anti-Sh serum. This contains the schematic localization of the most frequently immunolabeled cell bodies that was obtained with camera lucida drawing by moving throughout all focal planes of eight whole-mount brains. Open circles show the position of labeled cell bodies facing the ventral side of the brain, and solid circles represent cells occupying medial or dorsal positions. Red and blue spots correspond to neuroblasts and neurons, respectively. Black areas mark the location of MB neuropile, whereas shaded regions indicate total neuropile. Arrows mark the approximate positions of the semithin sections of E and G. E, Frontal section (4 µm) at medial level of the OL and central brain from a larval brain, immunostained, dehydrated, and embedded as described in Materials and Methods. Semithin sections were cut and counterstained with toluidine blue. Ventral is to the top; stars mark unstained axonal fibers. Arrow points to a labeled cell body. Photograph was taken at 400× magnification. F, Frontal section carried as in E at the level of thoracic segments. GC, Undifferentiated ganglion cells; MB, mushroom bodies; N, neuropile; OPC, outer proliferation center of the OL.
[View Larger Version of this Image (115K GIF file)]

To study the localization of the channels in more detail, we made serial semithin sections of immunostained larval brains and counterstained the somata with toluidine blue. This approach showed that the immunostaining is neither regular nor general throughout the neuropile (Fig. 1E,F). There are some areas clearly lacking in stain, such as the majority of transversal fibers that connect both hemispheres (Fig. 1E). It can also be observed that only a small number of cell bodies are actually immunostained (Fig. 1E,F). The labeling of cell bodies, particularly neuroblasts, was frequently found in intracellular locations (data not shown).

We have demonstrated previously by quantitative immunoblot assays that ~90% of Sh Kch in the adult fly are expressed in the head (Rogero and Tejedor, 1995). Therefore, we have approached the localization of these channels by serial sectioning and immunostaining of adult heads. In some cases, to improve the localization of the signal and its assignment to a given structure, immunolabeled sections were counterstained with toluidine blue.

The alpha -ShHX1 antiserum labels the retina, optic lobes (OL), and central brain throughout the whole head of the adult fly (Fig. 2A-E). The specificity of the immunolabeling again is demonstrated by the lack of any signal in the sections of Df flies (Fig. 2F). Sh Kch are observed in the following three general locations of the adult brain: neuropile, nerve fibers, and neuronal somata (Fig. 3). Examples of the first location include the wide distribution of immunostaining within the neuropile of the OL and central brain. However, the immunostaining is neither general nor homogeneous within each neuropile. As shown in Figures 2C-E and 3B, the pattern of immunostaining of the OL reveals the typical stratified tangential layers and the columnar organization of neuromeres that have been described extensively in Drosophila and other diptera (Ramon y Cajal and Sanchez, 1915; Strausfeld, 1976; Fischbach and Dittrich, 1989). Except the lamina, which lacks any signal, all OL neuromeres are labeled with varying intensity. At the medulla, layers 2 and 9 are highly labeled, whereas layers 4 and 6 show a lower intensity signal. The most distal layers of the lobula, all four layers of the lobula plate, and a fiber bundle located between the two, are also very strongly stained. In the central brain, the alpha , beta , and gamma  lobes of the MB exhibit the strongest labeling of neuropile regions (Fig. 2A), whereas the calices and peduncles stain weakly (data not shown). The entire neuropile of the central complex is also well-stained, whereas labeling of the antennal lobe is almost completely absent (Fig. 2B,J). The central brain structure, which shows the strongest staining, is a series of axonal tracks (Figs. 3A, Fig. 2C) that run transversely, connecting both sides of the ventrolateral protocerebrum (Strausfeld, 1976). Similarly, most main fiber tracks connecting different regions of the nervous system such as the anterior optic nerves, which connect the OL with the protocerebrum (Fig. 2D,G), the cervical fiber linking brain and thoracic ganglia (Fig. 2H), and the posterior optic track, which connects both OL (data not shown), were strongly stained. However, a striking exception is the first optic chiasm, which links lamina and medulla and, as shown in Figure 3B (star), lacks any immunostain. Leg nerves, generated by the axons of thoracic motoneurons that innervate leg muscles, are also extensively immunostained (Fig. 2I). We have also observed that most primary sensory afferents, including labro-frontal, ocellar nerves (data not shown), maxillo-labelar (Fig. 2E), antennal (Fig. 2A,J), and retinal inputs (see below), are also immunostained by the anti-Sh antiserum. Strong staining of thick fibers running all along the antennal nerve can be observed in a sagittal section of the head (Fig. 2J). Most, if not all, of these labeled antennal fibers bypass the antennal lobula, the neuropile of which lacks immunostaining, before reaching the brain. The antennal nerve is formed by two bundles of mechanosensory and chemosensory fibers that move together from the antenna until they reach the brain, where they split into two tracks. One bundle is the olfactory track, which terminates at the antennal lobe; the other is the antennal mechanosensory and motor center track, which bypasses the antennal lobe terminating at the mechanosensory region of the deuterocerebrum (Stocker RF et al., 1990). Accordingly, we have identified these labeled fibers as part of the antennal mechanosensory and motor center track.

Fig. 2. Immunolocalization of Sh Kch in the nervous system of adult flies. Serial frontal cryostat sections of 48-hr-old adult heads were immunostained as indicated in Materials and Methods. A-E, Every third or fourth immunostained frontal section taken from a series throughout a head of a w fly showing labeling of antennal nerves (AN); anterior optic nerves (AON); central complex neuropile (CC); lobula neuropile (LO); maxillo-labelar nerves (MLN); medulla neuropile (ME); alpha , beta , and gamma  lobes (a, b, and g, respectively) of the MB neuropile; retina (RE); and transversal fibers (TF). Lack of immunostaining of antennal lobula (AL) and lamina neuropile (LA) can be observed in B and E, respectively. F, Frontal section of an adult Df head at a level equivalent to that in C. Because this section completely lacks immunolabeling, the photograph was taken under Nomarski optics to make the tissue structure visible. The stained layer located between retina and lamina is the eye pigment of the basal lamina. G, High magnification showing anterior optic nerves connecting lobula (LO) and central brain (CB). H, Sagittal section at a medial plane through the head and thorax showing the brain including subesophagic ganglion (SEG), cervical fiber (CF), and thoracic muscles (TM). I, Sagittal section of a CS fly at the level of thoracic ganglia (TG) showing descending axons running along the leg nerve (LN). J, Sagittal section of a CS head at the level of the antenna (A). Beside the brain, other observable features are the strong labeling of antennal nerve (AN) and deuterocerebrum (DC). Notice that the antennal lobe (AL) is practically deprived of staining.
[View Larger Version of this Image (129K GIF file)]

Fig. 3. Different subcellular localization of Sh Kch in adult brain; counterstained sections. Cryostat sections of adult flies were immunostained with antiserum alpha -ShHX1 and counterstained with toluidine blue as described in Materials and Methods. A, High magnification of a counterstained section equivalent to that shown in Figure 2C showing the central brain at the level of transversal fibers. B, OL at 630× magnification in a horizontal section at a medial level in an adult w head. An arrowhead marks the position of third optic chiasm. Small arrows point to immunostained photoreceptor axons crossing the lamina nuclear layer. A large arrow points to a labeled axonal bundle located between lobula and lobula plate. Numbers in the medulla neuropile correspond to tangential layers described by Fischbach and Dittrich (1989) that are immunolabeled. Notice that although the first optic chiasm (marked with a star) lacks any DAB stain, it can be clearly detected because of the typical × shape that the nerve bundles produce by passing between toluidine blue counterstained cell bodies of the medulla cortex. C, Detail at 1000× magnification of a frontal section at the level of the fused body of the central complex, showing labeled cell bodies (arrows). FB, Fused body; La, lamina; Lo, lobula; Lp, lobula plate; Me, medulla; Oes, esophagus.
[View Larger Version of this Image (72K GIF file)]

In addition to the strong binding of anti-Sh antiserum to both neuropile and fiber tracks, we have also detected a third type of staining in the adult brain. This consists of staining of a small number of cell bodies that are spread throughout the cell body rind of the central brain (Fig. 3C) and OL (data not shown) with no reproducible pattern of distribution.

The expression of Sh Kch at the retina deserves particular attention. Each ommatidium of Drosophila is a precise assembly of 8 photoreceptors and 11 accessory cells in a honeycomb-like matrix (for review, see Wolf and Ready, 1993). A horizontal section of retina immunostained with alpha -ShHX1 shows a radial pattern of intense labeling (Fig. 4A). Because the staining is observed below the layer of the lens and pseudocones and extends beyond the basal membrane to the lamina nuclear layer, labeling of the cone and pigment cells is very unlikely. However, the staining of mechanosensory bristles that project from alternate facet vertices cannot be ruled out. To test this, we have used the mutant sc10.1, which lacks all external mechanosensory organs of the head including all retinal sensilla (García-Bellido et al., 1979; Campuzano et al., 1985). As shown in Figure 4B, the staining pattern of retina remains in sc flies. Therefore, this is most consistent with labeling of photoreceptor neurons. Despite their similarities, the eight photoreceptor cells from Drosophila ommatidia can be classified into four classes (R1,3,4,6; R2,5; R7; and R8) (Wolf and Ready, 1993). A tangential section of the retina shows that alpha -ShHX1 stains only the complete inner periphery of each ommatidium (Fig. 4C). Because the ommatidia structure is fully preserved under the fixation conditions used (Fig. 4E), it can be concluded that Sh Kch expressed in retina are specifically located at the outer membrane of all eight photoreceptor neurons.

Fig. 4. Expression and localization of Sh Kch at the retina. High-magnification views (630×) of immunostained horizontal cryostat sections of adult w (A) and sc (B) heads. Small arrows in A point to immunostained photoreceptor axons crossing the lamina nuclear layer. These cannot be observed in B because of the eye pigment of the basal lamina (arrowhead) of sc flies. C, Immunostained tangential cryostat section of a wt retina. D, Schematic representation of the cellular components of an ommatidium. E, Plastic tangential semithin section of a CS retina, prepared as described in Materials and Methods, showing the conservation of ommatidial structure. F, OL of an immunostained horizontal section of a sevenless head at a level equivalent to that in Figure 3B but without counterstaining. Br, Bristle; C, pseudocone; L, corneal lens; LA, lamina; ME, medulla; PC, pigment cell; R1-R7, photoreceptor neurons.
[View Larger Version of this Image (131K GIF file)]

The ommatidial structure of the insect eye generates a retinotopic projection in the OL, which is constructed in a columnar way. R1-R6 photoreceptors project to the lamina neuropile, whereas R7 and R8 axons cross the lamina through the first optic chiasm and synapse at the medulla neuropile (Strausfeld, 1976; Fischbach and Dittrich, 1989). Although the axons of photoreceptors are labeled when they leave the retina and cross the lamina nuclear layer, avoiding the neuronal cell bodies, the staining disappears as soon as they enter the lamina neuropile (Figs. 3B, 4A). On the other hand, the medulla exhibits strong immunostaining (Fig. 3B). This raises the question of whether R7 and R8 photoreceptors express Sh Kch at their synaptic terminals. To address this, we have immunostained sections of sevenless mutant flies, which lack R7 photoreceptors (Tomlinson and Ready, 1986), and have found that the intense immunolabeling of defined medulla layers in the wt OL (Fig. 3B) is not modified in the mutant (Fig. 4F). These results suggest the almost exclusive location of Sh Kch in the cell body and axonal membranes of R1-R7 photoreceptors, and a low occurrence, or absence, at their synaptic terminals in lamina and medulla.

Are Sh Kch splice variants expressed selectively in different brain regions?

Because the antiserum alpha -ShHX1 recognizes Sh isoforms equally (Rogero and Tejedor, 1995), genetic tools were applied to answer the question of whether different Sh Kch variants produced at the Sh locus by alternative splicing are expressed differentially at a cellular level. Three well-studied Sh mutants, T(X,Y)W32, T(X,Y)B55, and ShE62, which modify the repertoire of Sh splice isoforms, have been used to test whether Sh Kch expression is abolished in specific brain structures or group of cells. As shown in Figure 5A, W32 is a chromosomal translocation with the breakpoint located in the Sh transcription unit between exons 2 and 3 (Pongs et al., 1988; Schwarz et al., 1988). The W32 translocation does not preclude the expression of all Sh Kch (Hardie et al., 1991). We have shown in a previous study by using high-resolution bidimensional electrophoresis and immunoblot techniques that at least two major Sh Kch proteins expressed in the adult Drosophila brain were eliminated by this mutation (Rogero and Tejedor, 1995). The immunohistological analysis of W32 flies shows a general decrease in the intensity of CNS and retinal staining. This agrees with previous PCR experiments that showed that ShB was the most abundant Sh variant in the adult head (Hardie et al., 1991). Distinct brain areas of W32 flies, like most main fiber tracks (cervical fiber, anterior and posterior optic nerves, antennal nerves, and so forth), appear to show the same pattern of distribution as in wt. For example, the transversal fibers of the central brain can be compared in Figures 2C and 5B. However, clear differences between the W32 and wt patterns are also found. For example, it is remarkable that the strong labeling of the MB neuropile of wt brains (Fig. 2A) is almost completely eliminated in W32 (Fig. 5C). It must be emphasized that no ectopic distribution of immunolabeling was detected in any area of W32 CNS. This strongly suggests that the translocation W32 does not produce secondary alterations in the pattern of Sh Kch expression. The chromosomal translocation B55, because of its location between the two groups of 3' alternative exons (Pongs et al., 1988; Schwarz et al., 1988), in principle should eliminate the C-terminal type 1 isoforms without affecting type 2 isoforms (see Fig. 5A). However, B55 flies exhibited considerable ectopic expression of Sh Kch (data not shown), and therefore, this mutant was not used in this study. A good alternative to B55 is the mutant ShE62, which has a point mutation in the acceptor site of one of the 3' alternative splice variants (Lichtinghagen et al., 1990) and, accordingly, modifies only the type 1 C-terminal isoforms (see Fig. 5A). Although the expression of Sh Kch in many areas of the ShE62 nervous system, such as MB, central complex, retina, and so forth, does not seem to be modified by this mutation (data not shown), a few distinct features in the Sh Kch distribution can be found. The pattern of labeling of OL undergoes distinct changes in this mutant (Fig. 5D). For example, the staining of layers and columns seen in the wt medulla and lobula plate (Fig. 3B) is severely reduced and altered in ShE62 (Fig. 5D). A more evident change is the almost complete elimination of labeling at the antennal nerve (compare Figs. 2J and 5E), whereas primary sensory afferents and connective fibers (maxillo-labelar, optic nerves, leg nerves, and so forth) were not modified (data not shown). Together, these results indicate that differences in the distribution of Sh Kch between wt and W32 or ShE62 brains are attributable to the lack of expression in the mutant flies of Sh isoforms, which seem to be preponderantly expressed in a few defined areas.
Fig. 5. Changes in the distribution of Sh Kch in mutants with modifications in the repertoire of Sh splice variants. A, Schematic representation of the Sh transcription unit with the approximate location of B55, ShE62, and W32 mutations. B, Immunostained frontal cryostat section of an adult W32 head at a level equivalent to that of Figure 2C. C, Immunostained frontal cryostat section of a W32 head at the level of MB, equivalent to that in Figure 2A. D, Left hemisphere of an ShE62 adult head as seen from an immunostained horizontal section. Notice the marked decrease in the immunostaining of OL neuromeres relative to the strong retinal labeling when compared with an equivalent wt section (Fig. 3B). The arrow points to fibers crossing between the lobula and lobula plate, that appear to have a level of Sh Kch expression similar to that found in wt flies. Numbers in the medulla neuropile are as in Figure 3B. Notice that in contrast to the wt medulla, layer 4 has the strongest labeling, whereas layers 2 and 9 are very weakly stained. E, Immunostained sagittal section through the head of an ShE62 adult fly taken at a level equivalent to that in Figure 2J. A, Antenna; AL, antennal loula; AN, antennal nerves; LA, lamina; LO, lobula; LP, lobula plate; ME, medulla; MB, mushroom bodies; RE, retina; TF, transversal fibers.
[View Larger Version of this Image (106K GIF file)]

Late developmental expression of Sh Kch

We have shown in a previous work (Rogero and Tejedor, 1995) that the repertoire of Sh Kch splice variants expressed in embryo, larvae, and adult fly were rather different. Here, we have focused our attention on the second developmental wave of Sh Kch expression, because it is during this developmental period, from pupation to adult imago, that differentiation and definitive formation of the CNS structure occur (Kankel et al., 1980; Truman et al., 1993). We have analyzed, by immunoblot techniques, whether different Sh isoforms are expressed during metamorphosis and the beginning of imago life. As shown in Figure 6, changes in the pattern of detected proteins occur throughout this period, with a gradual increase in the relative intensity of larger MW bands, which are most abundant 48 hr after eclosion. This pattern remains stable at least for the next 72 hr (data not shown). Because we have shown previously that our procedures and control experiments preclude degradation of Sh proteins and that all protein bands detected by the antiserum alpha -ShHX1 are glycosylated to a similar extent (Rogero and Tejedor, 1995), it is unlikely that the complex Sh protein pattern shown in Figure 6 could be attributable either to proteolysis or to the maturation of a single protein caused by progressive glycosylation. To demonstrate that these changes in the electrophoretic pattern are a direct consequence of differential expression of Sh Kch splice variants, we have once again taken advantage of the mutant W32. As demonstrated previously in adult flies (Rogero and Tejedor, 1995), W32 mutants also eliminate a subset of the Sh isoforms expressed in CS flies late in development (Fig. 6, arrows). Interestingly, this subset comprises at least one Sh isoform, the expression for which is developmentally regulated (Fig. 6). Together, these experiments strongly suggest that changes in the developmental Sh protein pattern are primarily attributable to the differential usage of some of the Sh Kch splice variants eliminated by W32 (Fig. 5A, ShB, ShD). This also demonstrates that major changes in Sh band pattern actually occur after eclosion of the flies and, therefore, cannot be a consequence of neuronal development, because the CNS is considered to be fully formed and cells differentiated by this time (Kankel et al., 1980; Truman et al., 1993). Moreover, clear changes are detected when the fly is fully mature (8-48 hr). The question arises as to whether these band changes are the result of gradual substitution of isoforms expressed in a given structure or cell group during differentiation or of the de novo expression of Sh Kch that is required by a cell group during a given developmental period, or even a combination of both mechanisms. To answer this question, we have focused on structures such as retina, antennal nerve, leg motoneuronal fibers, and MB, which show strong expression of Sh Kch in the adult fly and are functionally related to biological activities that are beginning, or significantly increasing, after eclosion.
Fig. 6. Changes in the expression of Sh Kch isoforms during late development. Immunoblots of developmentally staged samples of CS and W32 flies from monodimensional SDS-PAGE gels. Experimental conditions were as published previously (Rogero and Tejedor, 1995). As indicated by the position of molecular weight standards, photographs show the region where, as demonstrated previously (Rogero and Tejedor, 1995), most Sh Kch proteins appear. LP, Late pupae; RE, recently eclosed fly; A7 and A48, adult flies 7 and 48 hr after eclosion. Arrowheads point to the position of an equivalent intense band in each blot, whereas arrows indicate the position of bands that disappear in W32 mutant flies.
[View Larger Version of this Image (31K GIF file)]

The expression of retinal Sh Kch occurs after the appearance of the visual pigment. The retina of P12 pupa (bright red eyes) does not show alpha -ShHX1 labeling (Fig. 7A). At the P14-P15 stage, a few hours before eclosion, labeling could be detected for the first time (Fig. 7B). In recently eclosed flies, immunostaining was intense (Fig. 7C), and during the first few hours of imaginal life, increased to the level found in the 48-hr-old retina. In contrast to the expression in retina, Sh Kch are detected from very early pupal stages at the OL neuropile (Fig. 7A) showing a pattern similar to that found in the adult brain (Fig. 2E). Thus, the expression of retinal Sh Kch appears to correlate with, or even slightly precede, the onset of sensory activity. Retina of flies, the late metamorphosis and manipulation of which were performed under dark conditions, shows a strong labeling (Fig. 7D), therefore excluding the possibility that light may trigger the expression of Sh Kch in photoreceptor cells.

Fig. 7. Changes of Sh Kch distribution during late development. A, Immunostained frontal section showing the right hemisphere of a CS P12 pupae at a level close to that shown in Figure 2E for an adult head. B, Idem for a P14-P15 pupae. C, Id for a recently eclosed fly. D, CS late third instar larvae were collected and pupation allowed to progress under normal conditions until P5. Development from P5 until ~48 hr after eclosion was performed in the dark. Flies were then collected and rapidly embedded (1-2 min) for immunohistology under red light, to which Drosophila photoreceptors are insensitive (Menne and Spatz, 1977). E, Sagittal section through the head of a CS P15 pupa at the level of the antennal nerve. This section is equivalent to that of Figure 2J. F, Id for a 7-hr-old imago. Notice the change in the relative intensities of brain and antennal nerve labeling when compared with E. G, Sagittal section of a CS P15 pupa at the level of the thoracic ganglia and leg nerves. H, Id for a recently eclosed fly. I, Immunostained frontal section of a CS P9 pupa at the level of MB. Abbreviations are as in Figure 2.
[View Larger Version of this Image (157K GIF file)]

At 18-20 hr after pupae formation, axons from differentiating antennal sensory neurons fasciculate and form the antennal nerve, which projects into the brain to complete the development of sensilla (Ray and Rodrigues, 1995). The expression of Sh Kch at the antennal nerve is first observed at the late pupal stage (P14-P15) as a weak staining (Fig. 7E) that increases in intensity after the eclosion of flies (Fig. 7F), reaching a plateau 24 hr later (data not shown). In contrast to changes in antennal nerves, general immunostaining of the brain does not vary much during this period (Figs. 7E,F, 2J).

Staining of axonal fibers from leg motoneurons is very weak at the late pupal stage (Fig. 7G), but becomes intense immediately after eclosion of the fly (data not shown), increasing to a maximum in the first few hours of imago life (Fig. 7 H).

In contrast to retina, antennal nerves, and leg nerves, Sh Kch expression at the MB is very high as early as P9 pupae (Fig. 7I) and is maintained throughout development (data not shown).

DISCUSSION

Diverse functional roles can be inferred from the distribution and localization of Sh Kch

This study shows a major localization of Sh Kch in defined synaptic regions and axons. This is consistent with the electrophysiological phenotype of Sh mutants that produces modifications in neurotransmitter release (Jan et al., 1977) and action potentials (Tanouye et al., 1981). The most intense expression of Sh Kch found in defined regions of the adult head such as MB and OL neuropile agrees with that found in an earlier immunohistological study (Schwarz et al., 1990). Although this previous work lacked analysis of many brain areas, there are some obvious differences with our results, such as the labeling of antennal lobe and lamina neuropiles and the lack of labeling of cell bodies and some axonal tracks reported by us. It is also striking that in the earlier study, antisera labeled a few nonspecific bands, but only a single specific band was detected in immunoblots of total Drosophila head proteins (Schwarz et al., 1990) in spite of the wide variety of different Sh splice variants generated at the Sh locus (Kamb et al., 1988; Pongs et al., 1988; Schwarz et al., 1988). Also, in the previous study, antisera could not detect Sh Kch in muscle cells, whereas our antiserum clearly labels postsynaptic Sh Kch at neuromuscular junctions (Tejedor et al., 1997). Thus, affinity and specificity deficits most probably can account for these contrasting results.

The preponderance of cellular localization of Sh Kch changes during development. In larval brains, Sh Kch are expressed at high levels throughout many synaptic areas and at low levels in some axonal fibers. By contrast, Sh Kch are abundant in most axonal fibers of the adult brain, whereas only a few synaptic regions appear to have these channels. This nonuniform localization in synaptic areas is supported further by comparison with the distribution patterns of synaptic proteins such as syntaxin (Cerezo et al., 1995), synaptotagmin, and synaptobrevin (DiAntonio et al., 1993). Together, this demonstrates a restricted expression of Sh Kch to certain neuronal populations, as suggested previously from electrical recordings performed in primary cultures (Baker and Salkoff, 1990) and studies performed with Sh transformant flies (Zhao et al., 1995).

Of particular interest is the high prevalence of Sh Kch in synaptic areas of lobula plate, MB, and central complex, structures implicated in integrative functions (Buchner et al., 1984; Heisenberg et al., 1985; Hanesch et al., 1989; Davis, 1993; Strauss and Heisenberg, 1993; Tully et al., 1994). The MB, for example, has been consistently related to associative olfactory learning (De Belle and Heisenberg, 1994). Because Sh Kch were not detected in the chemoreceptor axon fibers of the antennal nerve or in their synaptic connections at the antennal lobe, the altered olfactory behavior found in some Sh mutant alleles (Cowan and Siegel, 1986) must be attributable to the modified integration of sensory signals at the MB, rather than to abnormal transmission of the primary sensory signal. In the optic ganglia, Sh Kch are localized in a well-defined pattern. Schwarz et al. (1990) concluded that a single group of neurons (Y cells) could account for much of the Sh Kch pattern of expression in this tissue. However, this cannot be the case, because Y cells have been described as having no arborization endings at the distal medulla (Fischbach and Dittrich, 1989), where we have found two prominently labeled synaptic layers (layers 2 and 4). In contrast, our results favor the restriction of Sh Kch expression to a given retinotopic projection. Among the four different visual pathways that have been found in Drosophila (Bausenwein et al., 1992), most of the Sh Kch distribution at the OL fits very nicely with projections of pathway 2 neurons. This possible restricted expression may have interesting functional implications, because it has been suggested that different retinotopic projections are involved in the computation of color, shape, motion, and so forth (Buchner et al., 1984; Bausenwein et al., 1989).

The functional role of those Sh Kch found in neuronal cell bodies remains uncertain. Because we have frequently found them in intracellular locations, a transient expression or an intracellular pool of Sh Kch could be likely explanations. The rapid induction of Kch after certain stimuli and the short half-life of some Kch mRNAs (Takimoto et al., 1993) make this feasible. Interestingly, the relationship of voltage-sensitive Kch to the cell cycle has been reported extensively (for review, see Dubois and Rouzaire-Dubois, 1993). Thus, a transient expression of Sh Kch related to the cell cycle of neuroblasts is an attractive hypothesis.

Electrical recordings in Drosophila photoreceptors have found a Shaker current and two noninactivating K+ currents (Hardie, 1991). We have shown here that Sh Kch are located in the outer membrane and are absent from lumen and rhabdomere membranes. Because it has been suggested that the two non-Sh Kch are located in the internal lumen membranes (Hardie, 1991), Drosophila photoreceptors may provide a good model system to study the mechanisms involved in the cellular segregation of ion channels.

Sh Kch splice variants are expressed differentially but not completely segregated

The formation of heteromultimeric Kch by the assembly of different subunits has been proposed as a mechanism for the generation of Kch diversity (Isacoff et al., 1990; Ruppersberg et al., 1990). However, there is compelling evidence in the literature to support both the colocalization and the segregation of different Kch subunits in mammalian brain (Sheng et al., 1992, 1994; Wang et al., 1993, 1994; Scott et al., 1994; Mi et al., 1995; Weiser et al., 1995). PCR (Hardie et al., 1991), in situ hybridization (Tseng-Crank et al., 1991), and reporter gene engineering (Mottes and Iverson, 1995) experiments indicate that Sh splice variants can be expressed differentially in some areas of the nervous tissue, retina, and muscle of Drosophila. An immunohistological study on adult brain has shown that structures stained with an antiserum against a single Sh isoform were a subset of those labeled with a general anti-Sh antiserum (Schwarz et al., 1990), therefore suggesting a segregation of splice variants. However, it was not shown that the protein bands detected by WB with the isoform-specific serum were also a subset of the bands labeled by the general antiserum. Our experiments with mutants that selectively eliminate a few of the alternative Sh splice isoforms have shown that only in antennal nerve axons of the mutant ShE62 is the expression of Sh Kch apparently abolished. More typically, the expression is reduced by varying degrees in most brain regions of ShE62 and W32 flies. Therefore, it can be concluded that there is a wide differential usage of the repertoire of Sh splice variants, but that complete segregation takes place only in a few brain regions.

Differential spatio-temporal expression of Sh Kch isoforms and their role during late development

Large modifications of neuronal electrical properties during development have been recorded in various animals. Voltage-gated currents appear in a sequence characteristic of each neuronal population (for review, see Spitzer, 1991; Spitzer et al., 1994). Kch have been detected as early as neural induction (Ribera, 1990) and during development undergo abrupt changes in density and kinetics (Barish, 1986; Harris et al., 1988; Yool et al., 1988).

There are no reports in the literature on the differentiation of electrical properties of Drosophila CNS neurons, although some data are available from photoreceptor neurons (Hardie, 1991) and pupal muscle (Salkoff and Wyman, 1981). Previous work (Rogero and Tejedor, 1995) and results presented here clearly show that Sh Kch are expressed differentially throughout development of the Drosophila nervous system. In contrast to myotube differentiation, in which two Sh conductances with different electrical properties were recorded showing a progressive replacement of an early type IA by a late mature one (Broadie and Bate, 1993), we have shown that major changes in neuronal expression of Sh Kch during late development are not attributable to the replacement of Sh isoforms. Our results suggest a de novo expression of Sh isoforms that seems to correlate with the increase in sensory and motor activity of newborn flies. Thus, the expression of Sh Kch may be one of the last refinements in the differentiation of neuronal electrical properties and, in addition, may be involved in adaptative mechanisms of excitability, as suggested by the wide changes in the expression of Sh isoforms in adult flies.

FOOTNOTES

Received July 8, 1996; revised March 28, 1997; accepted April 10, 1997.

  

This work was supported by grants from the DGICYT, the Comunidad de Madrid, and the Generalitat Valenciana (F.J.T.), and a predoctoral fellowship of Comunidad de Madrid (O.R.). We thank M. J. Chuliá for expert technical assistance; S. Campuzano, A. Ferrús, and E. Hafen for fly stocks; and E. Buchner for introducing us to immunohistological techniques for fly heads. We also thank A. Ferrús, L. Iverson, and F. Moya for critically reading this manuscript.

Correspondence should be addressed to Dr. Francisco J. Tejedor, Instituto de Neurociencias, Unidad Asociada-Instituto Cajal-CSIC, Universidad de Alicante, San Juan, 03080 Alicante, Spain.


REFERENCES

  • Baker K, Salkoff L (1990) The Drosophila Shaker gene codes for a distinctive k current in a subset of neurons. Neuron 2:129-140.
  • Bainbridge SP, Bownes M (1981) Staging the metamorphosis of Drosophila melanogaster. J Embryol Exp Morphol 66:57-80[Web of Science][Medline].
  • Barish ME (1986) Differentiation of voltage-gated potassium current and modulation of excitability in cultured amphibian spinal neurones. J Physiol (Lond) 375:229-250[Abstract/Free Full Text].
  • Bausenwein B, Dittrich APM, Fischbach KF (1992) The optic lobe of Drosophila melanogaster. Cell Tissue Res 267:17-28[Web of Science][Medline].
  • Becker MN, Brenner R, Atkinson NS (1995) Tissue-specific expression of a Drosophila calcium-activated potassium channel. J Neurosci 15:6250-6259[Abstract].
  • Broadie KS, Bate M (1993) Development of larval muscle properties in the embryonic myotubes of Drosophila melanogaster. J Neurosci 13:167-180[Abstract].
  • Buchner E, Buchner S, Bulthoff H (1984) Identification of [3H]deoxyglucose-labelled interneurons in the fly from serial autoradiographs. Brain Res 305:384-388[Web of Science][Medline].
  • Buchner E, Buchner S, Crawford G, Mason WT, Salvaterra PM, Sattelle DB (1986) Choline acetyltransferase-like immunoreactivity in the brain of Drosophila melanogaster. Cell Tissue Res 246:57-62.
  • Budnik V, White C (1988) Catecholamine-containing neurons in Drosophila melanogaster: distribution and development. J Comp Neurol 268:400-413[Web of Science][Medline].
  • Campuzano S, Carramolino L, Cabrera CV, Ruiz-Gomez M, Villares R, Boronat A, Modolell J (1985) Molecular genetics of the achaete-scute gene complex of Drosophila melanogaster. Cell 40:327-338[Web of Science][Medline].
  • Cerezo JR, Jiménez F, Moya F (1995) Characterization and gene cloning of Drosophila syntaxin 1 (Dsynt 1): the fruit fly homologue of rat syntaxin 1. Mol Brain Res 29:245-252[Medline].
  • Cowan TM, Siegel RW (1986) Drosophila mutations that alter ionic conduction disrupt acquisition and retention of a conditioned odor avoidance response. J Neurogenet 3:187-201[Web of Science][Medline].
  • Davis RL (1993) Mushroom bodies and Drosophila learning. Neuron 11:1-14[Web of Science][Medline].
  • De Belle JS, Heisenberg M (1994) Associative odor learning in Drosophila abolished by chemical ablation of mushroom bodies. Science 263:692-695[Abstract/Free Full Text].
  • DiAntonio A, Burgess RW, Chin AC, Deitcher DL, Scheller RH, Schwarz TL (1993) Identification and characterization of Drosophila genes for synaptic vesicle proteins. J Neurosci 13:4924-4936[Abstract].
  • Dubois JM, Rouzaire-Dubois B (1993) Role of potassium channels in mitogenesis. Prog Biophys Mol Biol 59:1-21[Web of Science][Medline].
  • Fischbach KF, Dittrich APM (1989) The optic lobe of Drosophila melanogaster. I. A Golgi analysis of wild-type structure. Cell Tissue Res 258:441-475[Web of Science].
  • García-Bellido A (1979) Genetic analysis of the achaete-scute system of Drosophila melanogaster. Genetics 91:491-520[Abstract/Free Full Text].
  • Hanesch U, Fischbach K-F, Heisenberg M (1989) Neuronal architecture of the central complex in Drosophila melanogaster. Cell Tissue Res 257:343-366.
  • Hardie CR, Voss D, Pongs O, Laughlin SB (1991) Novel potassium channels encoded by the Shaker locus in Drosophila photoreceptor. Neuron 6:477-486[Web of Science][Medline].
  • Hardie RC (1991) Voltage-sensitive potassium channels in Drosophila photoreceptor. J Neurosci 11:3079-3095[Abstract].
  • Harris GL, Henderson LP, Spitzer NC (1988) Changes in densities and kinetics of delayed rectifier potassium channels during neuronal differentiation. Neuron 1:739-750[Web of Science][Medline].
  • Heisenberg M, Borst A, Wagner S, Byers D (1985) Drosophila mushroom body mutants are deficient in olfactory learning. J Neurogenet 2:1-30[Web of Science][Medline].
  • Hille B (1992) In: Ionic channels of excitable membranes. Sunderland, MA: Sinauer.
  • Isacoff EY, Jan YN, Jan LY (1990) Evidence for the formation of heteromultimeric potassium channels in Xenopus oocytes. Nature 345:530-534[Medline].
  • Iverson LE, Rudy B (1990) The role of the divergent amino and carboxyl termini on the inactivation properties of potassium channels derived from the Shaker gene of Drosophila. J Neurosci 10:2903-2916[Abstract].
  • Jan LY, Jan YN (1992) Tracing the roots of ion channels. Cell 69:715-718[Web of Science][Medline].
  • Jan LY, Jan YN (1994) Potassium channels and their evolving gates. Nature 371:119-122[Medline].
  • Jan YN, Jan LY, Dennis MJ (1977) Two mutations of synaptic transmission in Drosophila. Proc R Soc Lond [Biol] 198:87-108[Medline].
  • Kamb A, Tseng-Crank J, Tanouye M (1988) Multiple products of the Drosophila Shaker gene may contribute to potassium channel diversity. Neuron 1:421-430[Web of Science][Medline].
  • Kankel DR, Ferrús A, Garen SH, Harte PJ, Lewis PE (1980) The structure and development of the nervous system. In: The genetics and biology of Drosophila. Vol 2 (Ashburner M, Wright TRF, eds), pp 295-368. London: Academic.
  • Laemmli UK (1970) Cleavage of structural proteins during the assembly of the head of bacteriophagus T4. Nature 227:680-685[Medline].
  • Lichtinghagen R, Stocker M, Wittka R, Boheim G, Stühmer W, Ferrús A, Pongs O (1990) Molecular basis of altered excitability in Shaker mutants of Drosophila melanogaster. EMBO J 9:4399-4407[Web of Science][Medline].
  • Lundell MJ, Hirsh J (1994) Temporal and spatial development of serotonin and dopamine neurons in the Drosophila CNS. Dev Biol 165:385-396[Web of Science][Medline].
  • MacKinnon R (1991) Determination of the subunit stoichiometry of voltage-activated potassium channel. Nature 350:232-235[Medline].
  • Menne D, Spatz H-C (1977) Colour vision in Drosophila melanogaster. J Comp Physiol 114:301-312.
  • Mi H, Deerinck TJ, Ellisman MH, Schwarz TL (1995) Differential distribution of closely related potassium channels in rat Schwann cells. J Neurosci 15:3761-3774[Abstract].
  • Miller C (1991) 1990: Annus mirabilis of potassium channels. Science 252:1092-1096[Free Full Text].
  • Mottes JR, Iverson LE (1995) Tissue-specific alternative splicing of hybrid Shaker/lacZ genes correlates with kinetic differences in Shaker K+ currents in vivo. Neuron 14:613-623[Web of Science][Medline].
  • Pongs O (1992) Molecular biology of voltage-dependent potassium channels. Physiol Rev [Suppl] 72:S69-S88.
  • Pongs O, Kecskemethy N, Müller R, Krah-Jentgens I, Baumann A, Kiltz HH, Canal Y, Llamazares S, Ferrús A (1988) Shaker encodes a family of putative potassium channels in the nervous system of Drosophila. EMBO J 7:1087-1096[Web of Science][Medline].
  • Ramon y Cajal S, Sanchez D (1915) Contribución al conocimiento de los centros nerviosos de los insectos. Trab Lab Invest Biol 13:1-164.
  • Ray K, Rodrigues V (1995) Cellular events during development of the olfactory sense organs in Drosophila melanogaster. Dev Biol 167:426-438[Web of Science][Medline].
  • Ribera AB (1990) A potassium channel gene is expressed at neural induction. Neuron 5:691-701[Web of Science][Medline].
  • Rogero O, Tejedor FJ (1995) Immunochemical characterization and developmental expression of Shaker potassium channels from the nervous system of Drosophila. J Biol Chem 270:25746-25751[Abstract/Free Full Text].
  • Rudy B (1988) Diversity and ubiquity of K-channels. Neuroscience 25:729-749[Web of Science][Medline].
  • Rudy B, Kentros C, Vega-Saenz de Miera E (1991) Families of potassium channel genes in mammals. Toward an understanding of the molecular basis of potassium channel diversity. Mol Cel Neurosci 2:89-102.
  • Ruppersberg JP, Schröter KH, Sakmann B, Stocker M, Sewing S, Pongs O (1990) Heteromultimeric channels formed by rat brain potassium-channels proteins. Nature 345:535-537[Medline].
  • Salkoff L, Wyman R (1981) Genetic modification of potassium channels in Drosophila Shaker mutants. Nature 293:228-230[Medline].
  • Salkoff L, Baker K, Butler A, Covarrubias M, Pak MD, Wei A (1992) An essential "set" of K+channels conserved in flies, mice and humans. Trends Neurosci 15:161-166[Web of Science][Medline].
  • Schwarz TL, Tempel BL, Papazian DM, Jan YN, Jan LY (1988) Multiple potassium-channel components are produced by alternative splicing at the Shaker locus in Drosophila. Nature 331:137-142[Medline].
  • Schwarz TL, Papazian DM, Carretto RC, Jan YN, Jan LY (1990) Immunological characterization of K+-channel components from the Shaker locus and differential distribution of splicing variants in Drosophila. Neuron 4:119-127[Web of Science][Medline].
  • Scott VES, Muniz ZM, Sewing S, Lichtinghagen R, Parcej DN, Pongs O, Dolly JO (1994) Antibodies specific for distinct Kv subunits unveil a heterooligomeric basis for subtypes of alpha-dendrotoxin-sensitive K+ channels in bovine brain. Biochemistry 33:1617-1623[Medline].
  • Sheng M, Tsaur M-L, Jan YN, Jan LY (1992) Subcellular segregation of two a-type K+ channel proteins in rat central neurons. Neuron 9:271-284[Web of Science][Medline].
  • Sheng M, Tsaur M-L, Jan YN, Jan LY (1994) Contrasting subcellular localization of the Kv1.2 K+ channel subunit in different neurons of rat brain. J Neurosci 14:2408-2417[Abstract].
  • Spitzer CN (1991) A developmental handshake: neuronal control of ionic currents and their control of neuronal differentiation. J Neurobiol 22:659-673[Web of Science][Medline].
  • Spitzer NC, Gu X, Olson E (1994) Action potentials, calcium transients and the control of differentiation of excitable cells. Dev Biol 4:70-77.
  • Stocker M, Stuhmer W, Wittka R, Wang X, Muller R, Ferrus A, Pongs O (1990) Alternative Shaker transcripts express either rapidly inactivating or noninactivating K+channels. Proc Natl Acad Sci USA 87:8903-8907[Abstract/Free Full Text].
  • Stocker RF, Lienhard MC, Borst A, Fischbach KF (1990) Neuronal architecture of the antennal lobe in Drosophila melanogaster. Cell Tissue Res 262:9-34[Web of Science][Medline].
  • Strausfeld NJ (1976) In: Atlas of an insect brain. Berlin: Springer.
  • Strauss R, Heisenberg M (1993) A higher control center of locomotor behavior in the Drosophila brain. J Neurosci 13:1852-1861[Abstract].
  • Takimoto K, Fomina AF, Gealy R, Trimmer JS, Levitan ES (1993) Dexamethasone rapidly induces Kv1.5 K+ channel gene transcription and expression in clonal pituitary cells. Neuron 11:359-369[Web of Science][Medline].
  • Tanouye M, Ferrús A, Fujita SC (1981) Abnormal action potentials associated with the Shaker complex locus of Drosophila. Proc Natl Acad Sci USA 78:6548-6552[Abstract/Free Full Text].
  • Tejedor FJ, Bokhari A, Rogero O, Gorczyca M, Kim E, Sheng M, Bhandari P, Singh S, Budnik V (1997) Essential role for dlg in synaptic clustering of Shaker K+ Channels in vivo. J Neurosci 17:152-159[Abstract/Free Full Text].
  • Tomlinson A, Ready DF (1986) Sevenless: a cell specific homeotic mutation in the Drosophila eye. Science 231:400-402[Abstract/Free Full Text].
  • Truman JW, Taylor BJ, Timothy AA (1993) Formation of the adult nervous system. In: The development of Drosophila melanogaster (Bate M, Martinez-Arias A, eds), pp 1245-1276. New York: Cold Spring Harbour Laboratory.
  • Tseng-Crank J, Pollock JA, Hayashi I, Tanouye MA (1991) Expression of ion channel genes in Drosophila. J Neurogenet 7:229-239[Web of Science][Medline].
  • Tully T, Preat T, Boynton SC, Del Vecchio M (1994) Genetic dissection of consolidated memory in Drosophila. Cell 79:35-47[Web of Science][Medline].
  • Vallés AM, White K (1988) Serotonin-containing neurons in Drosophila melanogaster: development and distribution. J Comp Neurol 268:414-428[Web of Science][Medline].
  • Wang H, Kunkel DD, Martin TM, Schwartzkroin PA, Tempel B (1993) Heteromultimeric K+ channels in terminal and juxtaparanodal regions of neurons. Nature 365:76-79.
  • Wang H, Kunkel DD, Schwartzkroin PA, Tempel BL (1994) Localization of Kv1.1 and Kv1.2, two K channel proteins, to synaptic terminals somata, and dendrites in the mouse brain. J Neurosci 14:4588-4599[Abstract].
  • Weiser M, Bueno E, Sekirnjak C, Martone ME, Baker H, Hillman D, Chen S, Thornhill W, Ellisman M, Rudy B (1995) The potassium channel subunit Kv3.1b is localized to somatic and axonal membranes of specific populations of CNS neurons. J Neurosci 15:4298-4314[Abstract].
  • White K, Hurteau T, Punsal P (1986) Neuropeptide-FMRFamide-like immunoreactivity in Drosophila: development and distribution. J Comp Neurol 247:430-438[Web of Science][Medline].
  • Wolf T, Ready DF (1993) Pattern formation in the Drosophila retina. In: The development of Drosophila melanogaster (Bate M, Martinez-Arias A, eds), pp 1277-1326. New York: Cold Spring Harbour Laboratory.
  • Yool AJ, Dionne VE, Gruol DL (1988) Developmental changes in K+-selective channel activity during differentiation of the Purkinje neuron in culture. J Neurosci 8:1971-1980[Abstract].
  • Zhao M-L, Sable EO, Iverson LE, Wu C-F (1995) Functional expression of Shaker K+ channels in cultured Drosophila "giant" neurons derived from Sh cDNA transformants: distinct properties, distribution, and turnover. J Neurosci 15:1406-1418[Abstract].
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