Targeting the motor regulator Klar to lipid droplets
© Yu et al; licensee BioMed Central Ltd. 2011
Received: 1 December 2010
Accepted: 24 February 2011
Published: 24 February 2011
In Drosophila, the transport regulator Klar displays tissue-specific localization: In photoreceptors, it is abundant on the nuclear envelope; in early embryos, it is absent from nuclei, but instead present on lipid droplets. Differential targeting of Klar appears to be due to isoform variation. Droplet targeting, in particular, has been suggested to occur via a variant C-terminal region, the LD domain. Although the LD domain is necessary and sufficient for droplet targeting in cultured cells, lack of specific reagents had made it previously impossible to analyze its role in vivo.
Here we describe a new mutant allele of klar with a lesion specifically in the LD domain; this lesion abolishes both droplet localization of Klar and the ability of Klar to regulate droplet motion. It does not disrupt Klar's function for nuclear migration in photoreceptors. Using a GFP-LD fusion, we show that the LD domain is not only necessary but also sufficient for droplet targeting in vivo; it mediates droplet targeting in embryos, in ovaries, and in a number of somatic tissues.
Our analysis demonstrates that droplet targeting of Klar occurs via a cis-acting sequence and generates a new tool for monitoring lipid droplets in living tissues of Drosophila.
Lipid droplets are the intracellular sites for storage of neutral lipids. Long dismissed as inert inclusions, they are now recognized as dynamic organelles with a myriad of functions well beyond fat storage [reviewed in, , ]. In many cells, lipid droplets are highly motile, actively moving along cytoskeletal tracks . Such motion is implicated in the delivery of nutrients [4, 5], the growth and turnover of lipid droplets [6–8], the exchange of lipids and proteins between various cellular compartments [9–12], and even the assembly of viral particles .
Despite the ubiquity and potential biological significance of droplet motion, its mechanism is not well understood . Most characterized droplet motion occurs along microtubules, driven by motor proteins, such as the minus-end directed cytoplasmic dynein [8, 13–16] and the plus-end directed kinesin-1 . The same motor proteins are also employed in many other transport processes and are responsible for the motion of various vesicles, mitochondria, RNP particles, chromosomes and nuclei. Motion of these cargoes is regulated distinctly from that of lipid droplets [e.g., [18, 19]].
At least in part, specificity of droplet motion is achieved via distinct motor regulators that are present exclusively on lipid droplets. For example, in both mammals and flies, members of the Perilipin family modulate droplet motion [6, 13, 20]; these proteins localize largely or exclusively to lipid droplets . In Drosophila embryos, droplet motion is controlled by Klarsicht (Klar) , a protein highly enriched on lipid droplets at this stage of development . Presumably, unique motor regulators present only on droplets control specifically those motors attached to this cargo.
Klar's role is not limited to lipid droplets; in different cells, Klar controls distinct transport processes. In early embryos, it regulates the bidirectional motion of lipid droplets , which are transported by cytoplasmic dynein  and kinesin-1 . In embryonic salivary glands, in contrast, Klar is required for efficient transport of secretory vesicles , possibly by modulating the activity of cytoplasmic dynein. In developing photoreceptors, Klar promotes apical migration of nuclei . Motion of these nuclei is powered by cytoplasmic dynein , and also involves the activity of kinesin-1 . The intracellular localization of Klar reflects these varying functions in different tissues: in early embryos, Klar is present on lipid droplets ; in photoreceptors, it is enriched on the nuclear envelope [24, 27]. Apparently, Klar regulates the same or a similar set of motors in all these instances, and it is the location of Klar that determines which subset of cellular motors is controlled. Thus, determining how Klar is targeted intracellularly is a key to understanding its cargo specificity.
This tissue-specific targeting of Klar correlates with isoform variation . The klar locus encodes at least three protein isoforms that are due to the use of multiple promoters and Poly A sites . The alpha (α) isoform is required for nuclear migration in photoreceptors [22, 24]; the beta (β) isoform controls the motion of embryonic lipid droplets ; no function has yet been described for the gamma (γ) isoform. Because the α and β isoforms are predicted to have identical N-terminal regions of 1726 amino acids, but carry unique C-terminal regions (536 aa for Klar α, 114 aa for Klar β), these C-terminal domains may be cis-acting targeting sequences that dictate where in the cell Klar accumulates .
For Klar α, there is ample support for this model. Its C-terminal region contains a 60 aa KASH (Klarsicht/ANC-1/Syne Homology) domain. KASH domains typically localize to the outer nuclear envelope, and together with SUN domain proteins in the inner nuclear envelope establish a bridge linking cytoplasmic and nucleoplasmic proteins [28, 29]. Indeed, the KASH domain of Klar is sufficient to target unrelated proteins to the nuclear envelope, in cultured cells  as well as in photoreceptors . In addition, mutations of Klar α that truncate the protein within or just N-terminal to the KASH domain fail to localize to the nuclear envelope [22, 30]. Thus, the KASH domain is necessary and sufficient to target Klar to the nuclear envelope.
Available evidence is consistent with the notion that the unique C-terminal region of Klar β has an analogous role in targeting to lipid droplets. For example, in cultured cells, this so-called LD domain is sufficient to recruit RFP to lipid droplets . However, whether the LD domain is necessary and sufficient for droplet targeting in vivo has not been clearly established. For one, the exact distribution of LD fusion proteins in cultured cells is distinct from the distribution of endogenous Klar in vivo: in embryos, Klar β is present in one or a few dots per lipid droplet, suggesting that it may be recruited to privileged sites . In cultured cells, in contrast, RFP-LD fusions are evenly distributed all over the droplet surface, raising the possibility that targeting in the two systems occurs by distinct mechanisms. From mutational analysis, it is clear that in vivo droplet localization requires C-terminal regions of Klar β . However, all available klar alleles either only disrupt Klar α or truncate both Klar α and Klar β within the shared N-terminal region. Therefore, they cannot be used to distinguish if droplet targeting is due to the Klar β-specific LD domain or due to regions shared between Klar α and Klar β.
To examine the role of specifically the LD domain, we identified a new klar allele that deletes the last 64 aa of this domain. This allele abolishes droplet localization entirely. We also expressed a GFP-LD fusion protein and find that it targets to lipid droplets in early embryos, in the female germ line, and in somatic tissues. This analysis establishes that in vivo the LD domain is necessary and sufficient for targeting to lipid droplets.
Identifying a klar allele with a lesion in the LD domain
The transcripts for Klar α and β diverge after exon 15, followed either by exons 16, 17 and 18 (Klar α) or exon 15ext (Klar β) . Exon 15ext encodes the LD domain. Klar β proteins lacking C-terminal regions fail to localize to embryonic lipid droplets . All characterized klar alleles with lesions in Klar β remove not only the LD domain (114 amino acids), but also at least 128 amino acids encoded by exons 14 and 15, exons shared with Klar α. Thus, these reagents do not allow a conclusive test if targeting to embryonic lipid droplets requires the LD domain (unique to Klar β) or is mediated by regions common to both Klar α and Klar β.
To address this issue, we searched for new klar alleles with lesions specifically in the LD domain. Since Klar β null alleles are viable , we took advantage of a collection of EMS mutagenized, homozygously viable third chromosomes . We employed TILLING (Targeting Induced Local Lesions IN Genomes) [32–34] to find sequence changes in a genomic region that includes klar exon 15ext. We recovered two candidate lines (Z3-3772, Z3-1711) with predicted sequence changes in exon 15ext. We focused on the potential klar mutation in line Z3-3772 since it was predicted to result in deletion of roughly half of the LD domain.
To reconcile this observation with the TILLING results, we hypothesized that the mutation in the parental line might exist on the balancer chromosome, TM6B. We generated flies heterozygous for the TM6B chromosome from line Z3-3772 and for Df(3L)emc E12 , a large deletion that removes - among many other genes - the entire klar locus. Genomic sequencing revealed the absence of a contiguous 25 bp stretch in the middle of exon 15ext.
This deletion is not a general feature of the TM6B balancer chromosome. Although many of the lines from the mutant collection were analyzed as heterozygotes, the deletion was recovered only once. In particular, our screen identified sequence variations for 19 other lines for which DNA from heterozygous flies had been characterized; but for none of these lines was the 25 bp deletion identified. We also extracted a TM6B chromosome from a different stock of the collection and found that the 25 bp deletion was not present. Thus, this deletion in exon 15ext did not pre-exist on the TM6B chromosome and apparently arose spontaneously since the mutagenesis scheme employed to generate the collection  did not expose the balancer chromosomes to EMS. In the following, we will refer to the TM6B chromosome carrying this deletion as TM6BMW and to the corresponding klar allele as klar MW . The TM6B chromosome without this deletion and the corresponding klar allele will be called TM6BZ and klar Z , respectively.
What is the consequence of this change in the genomic sequence? The 25 bp deletion in exon 15ext shifts the open reading frame and should result in a truncated LD domain: While the initial 50 amino acids are unchanged, the C-terminal 64 residues are replaced by an unrelated five-amino-acid sequence (Figure 1A).
Predicted sequence variation in KlarMW
Ser to Thr
Ser to Thr
Ser to Ala
Asp to Glu
a, b, c
Ser to His
a, b, c
Thr to Ser
a, b, c
Ile to Asn
a, b, c
See Fig. 1A
Thr to Ser
Ser to Ala
The LD domain is necessary for droplet localization in vivo
The identification of klar MW provides an opportunity to test the functional consequences of disrupting the LD domain specifically. Although the other amino acid changes encoded by klar MW are likely benign, they could in principle be responsible for any phenotypes observed with klar MW . In the following, we therefore compare klar MW to the klar Z allele, which shares these changes, apart from the LD domain lesion.
To test if the mutant Klar was present on lipid droplets, we employed the assay previously used  to demonstrate that Klar is associated with embryonic lipid droplets: in-vivo centrifugation [11, 35]. When syncytial embryos are centrifuged, the major organelles sort out by density. In particular, lipid droplets accumulate on the side of the embryo that points up during centrifugation. In the wild type, this lipid-droplet layer is highly enriched for Klar; mutant Klar proteins that fail to target to lipid droplets are absent from this layer . We therefore determined Klar distribution in centrifuged embryos of various genotypes (Figure 2B). While in klar Z Klar was highly enriched on the droplet layer, Klar signal was absent from the droplet layer in the LD truncation mutant klar MW . We conclude that truncation of the LD domain abolishes targeting of Klar to lipid droplets. Thus, the LD domain is indeed necessary for droplet localization in vivo.
The LD domain truncation disrupts lipid-droplet transport in embryos
Klar β is important for the correct balance between plus- and minus-end motion. In the absence of Klar β, the global droplet distribution in Phases I and II is similar to the wild type, but becomes dramatically different in Phase III: lipid droplets remain around the center, instead of shifting back to the periphery. To assess if the LD domain contributes to Klar's function in this transport process, we compared klar MW and klar Z embryos. In both genotypes, the periphery turned clear in Phase II (not shown), just like for all other klar alleles previously characterized. In Phase III, klar Z embryos were opaque, like the wild type; a single copy of klar is indeed sufficient to support normal net droplet transport in Phase III . In contrast, klar MW embryos were clear, very similar to embryos lacking Klar β altogether (Figure 3B). This droplet mislocalization was confirmed by Nile Red staining (Figure 3A): In klar MW embryos, droplets accumulate around the central yolk in Phase II, and stay centrally in Phase III. Thus, klar MW behaves like a Klar β loss-of-function allele. We conclude that the LD domain is essential for Klar β function. Since it also disrupts the localization of Klar β to droplets, we conclude that proper targeting to droplets is necessary for Klar β to control droplet motion. Presumably, Klar β has to be in close proximity to the motors it regulates.
Sequence variation in the LD domain
The TILLING approach had uncovered a second strain (Z3-1770) with mutations in exon 15ext. We verified those changes by genomic sequencing; they are predicted to result in amino-acid changes at five positions (Figure 1A). In addition, in a survey of various laboratory strains, we found three amino-acid changes in Tai255.1, a stock collected from the wild in 1983. None of these changes apparently compromise Klar's function: In both strains, Klar localized to lipid droplets (data not shown), and lipid droplets displayed normal outward transport in Phase III (Figure 3B).
To identify other positions in the LD domain at which variation can be tolerated, we compared the sequence of this domain across seventeen fly species (Figure 1B). More than half of the LD domain displays dramatic sequence variation over this evolutionary time span (~250 Mya). But a 46 amino-acid stretch is highly conserved: 31 positions were either identical or similar among these species. This conservation suggests that this region is functionally important, likely for droplet targeting. This region is deleted in the non-targeting klar MW allele (arrow in Figure 1B).
The LD domain truncation supports nuclear migration in photoreceptors
Besides droplet transport, the best-characterized role of Klar is in the migration of nuclei in developing photoreceptors [19, 24]. Here, Klar localizes to the nuclear envelope , and has been proposed to act as an anchor for cytoplasmic dynein . Numerous lines of evidence suggest that this transport process requires the Klar α isoform [22, 24], but the available data do not clearly address if - in addition to Klar α - Klar β is also required to support nuclear migration. This uncertainty is in large part due to the fact that previously it was not possible to selectively abolish just Klar β function without also affecting Klar α [22, 27]. Klar MW now provides a unique opportunity to address if Klar β is required for proper positioning of photoreceptor nuclei.
A GFP-tagged LD domain localizes to embryonic lipid droplets
To determine the intracellular distribution of GFP-LD, we detected GFP fluorescence in living and in fixed embryos or stained fixed embryos with anti-GFP antibodies. All three methods revealed that the fusion protein was present in discrete puncta (Figure 5C, and data not shown), reminiscent of lipid droplets in size and abundance. These GFP-LD puncta moved actively, in a back-and forth manner (see the movies provided as Additional Files 1 and 2), similar to the bidirectional movement of lipid droplets . In addition, the global distribution of GFP signal also mimicked that of lipid droplets (Figure 5E). The generally peripheral distribution in Phase I was followed by accumulation around the central yolk in Phase II. In Phase III, GFP-LD was again broadly peripheral.
If GFP-LD indeed marks lipid droplets, its distribution should change predictably if lipid-droplet transport is altered. Inward transport of lipid droplets in Phase II requires the transport regulator Halo; in its absence, lipid droplets accumulate close to the plasma membrane, under the nuclei, rather than around the yolk in the center . Halo has no known role in the transport of any cargo beyond lipid droplets. In embryos lacking Halo, GFP-LD puncta also accumulate under the nuclei (Figure 5D), instead of around the yolk (Figure 5C). Furthermore, outward transport of lipid droplets in Phase III requires Klar β (Figure 3A). In the absence of endogenous Klar β, GFP-LD remained highly enriched in the yolk sack in Phase III (Figure 5E), just like lipid droplets [19, 22]. Thus, in these genotypes, GFP-LD distribution reflects the distribution of lipid droplets.
There are two unexpected patterns of the GFP-LD signal. First, it is present in fairly uniform rings, rather than the discrete spots observed for endogenous Klar β . Full-length Klar β might be restricted to certain regions on the droplet surface via interactions of the N-terminal region with other proteins. Alternatively, the binding partners that keep Klar β locally restricted may be limiting, present in lower amounts than the well expressed GFP-LD. Second, only some of the Nile-Red positive structures display strong GFP-LD signal (Figure 6C, D), while on others GFP levels were much weaker or barely detectable. It is striking that drastic intensity variations can be observed between neighboring lipid droplets in the same cell. This observation suggests that GFP-LD displays differential affinity to different droplets or that, once droplets are generated with distinct GFP-LD levels, GFP-LD does not readily exchange between droplets.
GFP-LD localizes to droplets in the absence of endogenous Klar β
The above analysis suggests that the LD domain is sufficient to target an unrelated protein to lipid droplets. This conclusion, however, might be misleading if the LD domain were a dimerization motif. In that case, GFP-LD could physically interact with full-length Klar β and would be targeted to lipid droplets secondarily, even if full length Klar were to bind to the droplets via other domains. Although the analysis of klar MW makes this possibility unlikely, we performed a rigorous test of this idea by examining GFP-LD in a Klar β null background. GFP-LD was still present in distinct cytoplasmic rings the size of lipid droplets (Figure 5F) that moved bidirectionally (not shown). In addition, global GFP-LD distribution followed that of lipid droplets: throughout the periphery in Phase I, and accumulated in or around the central yolk in Phases II and III (Figure 5E). Thus, GFP-LD localization to lipid droplets does not require endogenous Klar β.
The GFP-LD fusion co-purifies with lipid droplets
Lipid droplets are rich in neutral lipids and have a low buoyant density. This property makes it possible to biochemically separate droplets from other cellular structures. We therefore asked if GFP-LD copurifies with lipid droplets. In a first test, we employed in-vivo centrifugation of intact embryos . In such centrifuged embryos, GFP-LD signal was highly enriched in the lipid-droplet layer (Figure 6A), just like endogenous Klar (Figure 2B). This enrichment is not due to the GFP portion as many other GFP fusion proteins are excluded from the droplet layer in this assay . It also does not depend on endogenous Klar β since GFP-LD was enriched in the droplet layer in the Klar β null background (Figure 6A). Second, we lysed embryos and enriched for droplets using a sucrose step-gradient (Figure 6B). The top, lipid-droplet fraction was highly depleted for the cytoplasmic protein tubulin and greatly enriched for the bona-fide lipid-droplet protein LSD-2. GFP-LD was similarly enriched in this fraction. Taken together, these two approaches demonstrate that GFP-LD co-purifies with lipid droplets and provide independent evidence that the LD domain is sufficient to target an unrelated protein to lipid droplets.
The LD domain mediates droplet localization in many cell types
How proteins are targeted to lipid droplets is not well understood . Droplet-localized proteins fall into two broad classes. Some proteins localize to lipid droplets in essentially all cells they are expressed in, such as the Perilipin family members PLIN1and PLIN2 (formerly called Perilipin and ADRP, respectively) [21, 38]. This constitutive localization is in contrast to the conditional recruitment of, e.g., hormone-sensitive lipase; this enzyme moves from a general cytoplasmic distribution to the surface of lipid droplets in response to hormonal signaling . In addition, specific proteins from other cellular compartments localize to lipid droplets only in certain developmental stages or under specific environmental conditions . For early embyronic droplets in Drosophila, certain histones are such conditional lipid-droplet proteins ; many more proteins potentially behave similarly as the proteomes of embryonic and of fat-body droplets show considerable differences [11, 41]. We therefore asked whether localization of GFP-LD occurs only in early embryos or is a general phenomenon.
Using the ubiquitously active Act5C-Gal4 driver, we also expressed GFP-LD in somatic cells. In a number of adult and larval tissues, we found discrete GFP puncta, including in follicle cells in the adult ovary, larval salivary glands, and imaginal discs. These structures are lipid droplets, as they appear as rings at higher magnification and co-label with Nile Red (Figure 7D, E, F). Since in the wild type lipid droplets are abundant in certain imaginal discs , in follicle cells (MAW, unpublished observations), as well as in nurse cells and oocytes , GFP-LD likely does not induce lipid storage de-novo in these tissues, but localizes to pre-existing droplets.
In summary, targeting of the LD domain to lipid droplets is not an embryo-specific phenomenon. GFP-LD also localizes to lipid droplets in the female germ line and in a number of somatic tissues. In addition, an analogous RFP-LD fusion protein localizes to lipid droplets in cultured Drosophila cells . Thus, GFP-LD is not a conditional droplet protein, and the mechanism targeting the LD domain to lipid droplets is quite general.
A klar allele specific for the Klar β isoform
Because the klar locus encodes at least three proteins with different exon content, different lesions in klar have distinct effects on the isoforms and thus on distinct biological processes . Lesions in exons 0 through 15 disrupt both Klar α and Klar β; these so-called class I alleles impair both nuclear migration in photoreceptors and motion of embryonic lipid droplets. Lesions in exons 16 through 18 disrupt Klar α and Klar γ; such class II alleles impair nuclear migration, but not droplet motion. The new allele klar MW disrupts Klar β but not Klar α; it alters droplet motion but not nuclear migration. It constitutes a new type of allele (class III) that selectively impairs the β isoform.
Klar MW provides a unique tool to separately examine the functions of Klar α and Klar β. Klar is widely expressed  and has been implicated in a number of biological processes beyond droplet motion and nuclear migration [23, 44–48]. In most cases, it is unknown which Klar isoform is involved. The combination of class I, II and III alleles should make it possible to disentangle this functional complexity.
Droplet targeting by the LD domain
Our analysis of GFP-LD fusions suggests that targeting of Klar β to lipid droplets is a multi-step process. In many cells, GFP-LD strongly accumulates on lipid droplets (Figure 6, 7). In mid-stage oocytes, in follicle cells, and in the salivary gland, GFP fluorescence is also detected diffusely and in membranous structures and tubules reminiscent of the nuclear envelope or the ER (not shown). Under sensitive imaging conditions, similar additional GFP-LD distribution becomes apparent also in early embryos. These observations suggest that - in addition to strong affinity to lipid droplets - GFP-LD has a weak affinity to certain membranous compartments. We do not know yet whether this additional localization represents nascent GFP-LD in transition to lipid droplets, ectopic localization due to high levels of expression, or genuine multiple targeting. Dual localization of proteins to both the ER and lipid droplets is common, presumably because lipid droplets originate from the ER .
Nevertheless, GFP-LD clearly accumulates strongly on lipid droplets in many tissues, forming characteristic ring structures. Intriguingly, this distribution is distinct from the distribution of full-length Klar β, which is present in discrete dots on embryonic droplets , a distribution similar to that of the motor dynein ; thus, full-length Klar may be recruited to distinct spots by physical interactions with microtubule motors. GFP-LD may not be restricted to such dots because interactions with the motors might require sequences in the N-terminal region of Klar β or because GFP-LD is overexpressed relative to its interaction partners. We favor the former explanation since even those lipid droplets with comparatively low GFP-LD signal show a ring-like distribution of GFP-LD (Figure 6C, D). In the future, these hypotheses can be distinguished by comparing the distribution of GFP-LD and GFP-Klar β expressed at similar levels.
What is the molecular mechanism by which the LD domain, a region just 114 amino acids in length, is recruited to lipid droplets? Evolutionary conservation and mutational analysis point to a 46 amino acid region as critical for targeting (Figure 1B). Many proteins localize to droplets via hydrophobic targeting motifs thought to insert into the phospholipid monolayer surrounding droplets and to make contacts with the hydrophobic core. Examples include the proline knot motif of plant oleosins , hydrophobic patches in caveolin  or amphipathic helices in various Perilipin family members . Consistent with this possibility, the 46 aa conserved region of the LD domain is fairly hydrophobic (light blue residues in Figure 1B) and the regular interspersion of charged residues is compatible with this region forming an amphipathic helix (Figure 1C). Alternatively, this motif may allow the LD domain to physically interact with resident droplet proteins, e.g. just like hormone-sensitive lipase is recruited to droplets by binding to PLIN1 . If so, the binding partners of the LD domain cannot be exclusive to embyronic droplets since droplet targeting occurs in many types of cells (Figure 7). As a first step towards uncovering the targeting mechanism, a structure-function analysis of this region should reveal which features of the sequence (e.g., general hydrophobicity versus specific residues) are essential for proper droplet targeting. These studies can be conducted in the more accessible cultured-cell system, since the LD domain shows the same targeting properties in vivo (Figure 6, 7) as in cultured cells .
Since GFP-LD localizes to the droplet surface, it might potentially interfere with lipid metabolism. For example, in cultured mammalian cells, overexpression of PLIN2 promotes lipid-droplet accumulation, presumably by shielding the droplets from access by lipases [51, 52]. We have not noticed dramatic effects on lipid storage upon GFP-LD overexpression. Total triglyceride levels in wild-type and GFP-LD expressing embryos are very similar (Figure 5G), and in a range of cell types, lipid droplets carrying high levels of GFP-LD are very similar in size to nearby droplets with low GFP-LD levels (Figure 6 and 7). These data do not rule out that GFP-LD causes minor quantitative changes in lipid storage or only produces effects in specific cell types or under certain physiological conditions.
Why is GFP-LD distribution not uniform?
It is striking that not all lipid droplets accumulate GFP-LD to the same level. Lipid droplets in close proximity in the same cell can have dramatically different GFP-LD signal (Figures 6, 7). An exciting development in recent years has been the realization that not all lipid droplets within a given cell are identical; in particular, they can carry different proteins [37, 38, 41, 53]. However, the lipid droplets in early Drosophila embryos appear quite uniform, in size distribution and motile behavior [14, 18, 19]; droplet proteins previously examined displayed no obvious variation between droplets [11, 20]. To our knowledge, the uneven distribution of GFP-LD is the first hint that different embyronic droplets might have distinct properties.
Currently, we cannot distinguish whether GFP-LD is preferentially recruited to certain types of droplets existing naturally or whether GFP-LD expression causes differences between droplets. For example, Gal4 drivers often show mosaic expression in nurse cells ; and we sometimes observed, in the same egg chamber, nurse cells with variable GFP-LD expression (data not shown). Droplets that originated in different nurse cells may therefore carry distinct levels of GFP-LD once they reach the oocyte. We suspect that such mosaic expression does not fully account for the differential labeling because we observe drastic variation in GFP-LD levels also between droplets in single nurse cells as well as in other cells (Figure 7).
The role of the LD domain for droplet transport
The LD domain is necessary not only for droplet localization of Klar β, but also for Klar β's function in regulating droplet transport. Our results indicate that although the LD domain is sufficient for droplet localization, by itself it does not mediate Klar's transport functions. When expressed in the Klar β null background, most GFP-LD signal remains in the yolk sack in Phase III (Figure 5E). In addition, Klar β null embryos remain clear in Phase III, whether or not they express GFP-LD (Figure 3B). Simply targeting GFP-LD to lipid droplets is apparently not sufficient to restore Klar β's function.
Although it is conceivable that GFP-LD expression levels were simply not high enough for rescue of the transport defects, we disfavor this explanation since a full-length, GFP-tagged Klar β construct expressed at much lower levels is sufficient to profoundly alter droplet motion (YVY and MAW, unpublished observations). We therefore conclude that proper regulation of droplet motors requires the N-terminal region of Klar β and not just the LD domain. This model is further supported by the fact that Klar α shares those N-terminal regions and is also involved in motor regulation.
Whether the LD domain simply targets Klar β to lipid droplets or has additional functions is not yet clear. For example, because in yeast the LD domain can interact with the droplet protein LSD-2, it has been suggested that it participates in transmitting developmental signals from LSD-2 via Klar to motors . In the future, it will be interesting to investigate whether expression of GFP-LD alters subtle aspects of droplet motion, e.g., the exact distances traveled in a single run or the frequency of pausing .
However, our data suggest that such effects, if they exist at all, do not alter the net outcome of transport. GFP-LD expressing embryos displayed the same transparency changes as the wild type: the embryo periphery became transparent in Phase II and cloudy in Phase III (Figure 3B, and data not shown). Also, in the presence of GFP-LD, inward droplet transport in Phase II still depends on Halo (Figure 5D) and outward droplet transport in Phase III depends on endogenous Klar β (Figure 5E), just as for embryos not expressing the fusion protein . These conclusions hold true whether we examine transparency changes in the embryos (to reveal the behavior of the entire droplet population) or GFP fluorescence directly (Figure 3B; Figure 5D, E).
Since LD has the ability to bind to lipid droplets in a wide range of cells, Klar β may control droplet motility in many tissues. In Drosophila, droplet motion has so far been described only in early embryos  and in oocytes , but no systematic analysis has been conducted. New GFP fusions to mark lipid droplets in vivo[37, 56], including the GFP-LD constructs described here, will make it possible to address to what extent droplets move in other tissues and whether disruption of Klar β alters that movement.
To test the function of the LD domain of Klar β, we generated inducible GFP-LD fusion constructs and identified a klar allele that specifically disrupts the LD domain. Using these tools, we demonstrate that the LD domain is both necessary and sufficient for droplet targeting in vivo. We conclude that Klar β is targeted to lipid droplets via an isoform-specific protein motif, just like Klar α is targeted to the nuclear envelope via the KASH domain. Thus, it is controlled inclusion of cis-acting targeting sequences that mediates the differential intracellular localization of Klar in distinct tissues. Although Klar's LD domain is necessary for Klar β to act in the regulation of lipid-droplet transport, by itself it does not mediate Klar's transport functions. Likely it is the N-terminal regions shared between Klar α and Klar β that mediate motor regulation. In this model, variable C-terminal targeting sequences control Klar's intracellular distribution and thus dictate which subset of intracellular motors is controlled by Klar.
Oregon R was used as the wild-type stock. The stocks carrying klar alleles klar YG3 and klar 1 and the deficiency Df(3L)emc E12 were described previously [19, 22]. The collection of mutagenized third chromosomes was generated by the Zuker laboratory . Line Z3-1711 might represent a different chromosome than the others from the collection: it did not display the recessive eye color markers characteristic for these stocks , and it had five simultaneous amino-acid changes in the LD domain (Figure 1A). However, for the purposes of the analysis described here, the exact origin of this chromosome is not important. The critical information is the presence of these mutations in the LD domain and the wild-type phenotype for droplet transport and Klar localization. Tai255.1 is a wild-type D. melanogaster strain isolated in 1983 at Ivory Coast ; it displays normal net droplet transport .
To generate the GFP-LD expressing flies, GFP was amplified from pEGP-C1 (Clontech) and cloned into the Kpn I and Not I sites of pUASp . A tobacco etch virus (TEV) protease site (GAGAATTTGTATTTTCAGGGT) was generated by oligo nucleotide synthesis and cloned 3' to the GFP gene. The LD domain was amplified from cDNA clone LD08331  and cloned in frame 3' to the TEV site. The resulting plasmid was injected into Drosophila embryos by Genetic Services, Inc. (Cambridge, MA). Transgenic flies were selected by eye color. In total, twenty lines mapping to the X, second or third chromosome were established. To express the fusion proteins, transgenic animals were crossed with lines carrying matβ4-Gal4-VP16 or Act5C-Gal4 drivers.
TILLING, genomic sequencing, and sequence analysis
TILLING analysis was performed by the Fly-TILL service as described . In ~6000 strains from the Zuker collection , we screened a 1519 bp genomic region from the end of exon 12 through the coding region of exon 15ext. Nucleotide changes were uncovered in 23 lines; in two cases (Z3-1711 and Z3-3772), these changes mapped to exon 15ext. For these two strains, we sequenced PCR products encompassing exon 15ext as described below. The nucleotide changes observed in line Z3-3772 were due to changes on the balancer chromosome (see main text for details).
DNA primers were created to bookend individual exons of klar piecemeal using annealing temperatures and GC content to determine the most effective oligo sequences (primer sequences available upon request). Purified DNA from adult flies was used to individually PCR amplify these genomic fragments. PCR products were depleted of free nucleotides with ExoSAP-IT and sequenced at the Life Sciences Core Laboratories Center at Cornell University. Sequencing results were compared to the canonical sequences available on FlyBase.
To determine the pattern of evolutionary conservation in the LD domain, we first identified the likely klar exon 15 in the available genome annotations for the Drosophila and mosquito species accessible via the FlyBase BLAST server. We also identified related sequences from the G. morsitans genome project (Sanger Institute) as well as in a cDNA from the medfly C. capitata (GenBank # FG077614.1). In Drosophila melanogaster, exon 15ext follows immediately downstream of exon 15. In all 16 additional fly species examined, the corresponding DNA sequences downstream of exon 15 have the potential to encode proteins with significant similarity to the D. melanogaster LD domain (Figure 1B). These protein sequences were aligned with Clustal2.
In-vivo centrifugation, fixation, immunostaining, and imaging
Living embryos were centrifuged to separate lipid droplets from other cellular components, as described . Embryos were either embedded in agar to keep them in a fixed orientation during centrifugation, or they were centrifuged in random orientations in microcentrifuge tubes filled with buffer, and the lipid-droplet layer was identified by its characteristic appearance by bright-field microscopy. To separate organelles by density in oocytes and nurse cells, females were centrifuged in buffer-filled microfuge tubes as described .
To stain lipid droplets, dechorionated embryos or dissected fly tissues were fixed in 4% formaldehyde in PBS for 10-15 min using standard procedures [59, 60]. For embryos, this treatment is sufficient to make the vitelline membrane permeable to Nile Red. After washing, these samples were suspended with 1% BSA in PBS and stained with Nile Red at 20 μg/ml. In some cases (Figure 7D, E, F), unfixed tissues were directly stained with Nile Red. For immunodetection of GFP or Klar, dechorionated embryos were heat fixed and devitellinized using standard heptane-methanol procedures [59, 60]. They were stained either with mouse monoclonal Klar-M as described  or with rabbit anti-GFP (Torrey Pines Biolabs) at 1:10,000. Before use, the anti-GFP antibody was exposed to heat-fixed wild-type embryos to remove cross-reacting antibodies.
Two approaches were employed to examine GFP-LD fluorescence in living embryos. For confocal microscopy, embryos were hand-dechorionated, placed in halocarbon oil on a glass slide, and covered with a cover glass that was supported by spacers. For epifluorescence microscopy, embryos were placed into halocarbon oil on a glass slide. The halocarbon oil turns the chorion transparent (see Figure 3B).
Micrographs were acquired on a Leica SP5 confocal microscope or a Nikon Eclipse E600 fluorescence microscope with a 4MP Spot Insight camera. Images were processed in Adobe Photoshop and assembled with Adobe Illustrator.
For Western analysis, proteins were typically separated on a 10% SDS PAGE gel and transferred to PVDF membranes using standard Towbin or CAPS transfer. Mouse anti- alpha tubulin (Sigma-Aldrich) was used at 1:10,000, and mouse anti-GFP (Roche) at 1:1000. LSD-2 was detected with a rabbit polyclonal anti-serum  at 1:20,000. To consistently detect Klar β, this general procedure was optimized: Proteins were separated on 6% gels, and transferred in 25 mM Tris, 192 mM glycine, 10% methanol, 0.01% SDS to PVDF membranes (2 hrs at 100 V). Membranes were sequentially exposed to Klar-M (1:50, overnight at 4°C), rat anti-mouse IgG (1:1000; 1 hr at room temperature) and HRP-conjugated goat anti-rabbit IgG (1:1000; 1 hr at room temperature).
To generate samples enriched in lipid droplets, we adapted the protocol described previously . For each genotype, 150 μl of embryos (0-3 hrs old) were dechorionated, resuspended in 300 μl TKM (50 mM Tris, pH 7.4, 25 mM KCl, 5 mM MgCl2) containing 1 M sucrose plus protease inhibitor cocktail (Sigma-Aldrich), and then mechanically disrupted on ice. The lysate was transferred to a fresh 1.5 ml tube and overlaid sequentially with 200 μl TKM containing 0.5 M sucrose, 200 μl TKM containing 0.25 M sucrose, and 400 μl TKM. After centrifugation at 1000 g for 5 min, 5000 g for 5 min and 13400 g for 10 min, the buoyant lipid droplets were collected from the top of the gradient. The amount of protein in the isolated lipid droplets was measured by Bradford protein assay (Quick Start, Bio-Rad) before solubilizing the lipid droplets in SDS-containing buffer for subsequent SDS-PAGE analysis. Fractions such prepared are similar to those described by Cermelli et al. : the overall pattern of major Coomassie-stainable proteins is similar; the droplet protein LSD-2 and several histones are consistently enriched, and the cytoplasmic protein tubulin is absent (Figure 6B; Li and Welte, unpublished observations).
Embryos were collected for 1.5 hr, dechorionated with 50% bleach, and resuspended in triton salt solution [59, 60]. 200 embryos before cellularization stages were handselected, resuspended in 200 μl homogenizing buffer (0.01 M KH2PO4, 1 mM EDTA, pH 7.4), and mechanically disrupted. 40 μl of this lysate were mixed with 1 ml activated Triglyceride Reagent (Liquicolor Triglycerides, Stanbio), and triglyceride levels were determined according to the manufacturer's instructions. For each experiment, three independent samples were analyzed per genotype, and the data shown in Figure 5G are based on two independent experiments.
We thank the Bloomington Drosophila stock center for fly stocks, the Drosophila TILLING Project for performing the TILLING analysis, and the Zuker laboratory for generating and sharing the mutagenized third chromosome lines. We are grateful to Matthew Brockway and Joshua Geiger for help with immunostaining and sequencing, and to Gurpreet Arora for critical reading of the manuscript. This work was supported by start-up support from the University of Rochester and NIGMS grant GM64687 to MAW.
- Farese RV, Walther TC: Lipid Droplets Finally Get a Little R-E-S-P-E-C-T. Cell. 2009, 139: 855-860. 10.1016/j.cell.2009.11.005.PubMed CentralView ArticlePubMedGoogle Scholar
- Martin S, Parton RG: Lipid droplets: a unified view of a dynamic organelle. Nat Rev Mol Cell Biol. 2006, 7: 373-378. 10.1038/nrm1912.View ArticlePubMedGoogle Scholar
- Welte MA: Fat on the move: intracellular motion of lipid droplets. Biochem Soc Trans. 2009, 37: 991-996. 10.1042/BST0370991.View ArticlePubMedGoogle Scholar
- Bago B, Zipfel W, Williams RM, Jun J, Arreola R, Lammers PJ, Pfeffer PE, Shachar-Hill Y: Translocation and utilization of fungal storage lipid in the arbuscular mycorrhizal symbiosis. Plant Physiol. 2002, 128: 108-124. 10.1104/pp.010466.PubMed CentralView ArticlePubMedGoogle Scholar
- Cocchiaro JL, Kumar Y, Fischer ER, Hackstadt T, Valdivia RH: Cytoplasmic lipid droplets are translocated into the lumen of the Chlamydia trachomatis parasitophorous vacuole. Proc Natl Acad Sci USA. 2008, 105: 9379-9384. 10.1073/pnas.0712241105.PubMed CentralView ArticlePubMedGoogle Scholar
- Marcinkiewicz A, Gauthier D, Garcia A, Brasaemle DL: The phosphorylation of serine 492 of perilipin A directs lipid droplet fragmentation and dispersion. J Biol Chem. 2006, 281: 11901-11909. 10.1074/jbc.M600171200.View ArticlePubMedGoogle Scholar
- Nagayama M, Uchida T, Gohara K: Temporal and spatial variations of lipid droplets during adipocyte division and differentiation. J Lipid Res. 2007, 48: 9-18. 10.1194/jlr.M600155-JLR200.View ArticlePubMedGoogle Scholar
- Andersson L, Boström P, Ericson J, Rutberg M, Magnusson B, Marchesan D, Ruiz M, Asp L, Huang P, Frohman MA, Boren J, Olofsson SO: PLD1 and ERK2 regulate cytosolic lipid droplet formation. J Cell Sci. 2006, 119: 2246-2257. 10.1242/jcs.02941.View ArticlePubMedGoogle Scholar
- Goodman JM: The gregarious lipid droplet. J Biol Chem. 2008, 283: 28005-28009. 10.1074/jbc.R800042200.PubMed CentralView ArticlePubMedGoogle Scholar
- van Manen HJ, Lenferink A, Otto C: Noninvasive Imaging of Protein Metabolic Labeling in Single Human Cells Using Stable Isotopes and Raman Microscopy. Anal Chem. 2008, 80: 9576-9582. 10.1021/ac801841y.View ArticlePubMedGoogle Scholar
- Cermelli S, Guo Y, Gross SP, Welte MA: The lipid droplet proteome reveals that droplets are a protein storage depot. Curr Biol. 2006, 16: 1783-1795. 10.1016/j.cub.2006.07.062.View ArticlePubMedGoogle Scholar
- Zehmer JK, Huang Y, Peng G, Pu J, Anderson RG, Liu P: A role for lipid droplets in inter-membrane lipid traffic. Proteomics. 2009, 9: 914-921. 10.1002/pmic.200800584.PubMed CentralView ArticlePubMedGoogle Scholar
- Boulant S, Douglas MW, Moody L, Budkowska A, Targett-Adams P, McLauchlan J: Hepatitis C Virus Core Protein Induces LIpid Droplet Redistribution in a Microtubule- and Dynein-Dependent Manner. Traffic. 2008, 9: 1268-1282. 10.1111/j.1600-0854.2008.00767.x.View ArticlePubMedGoogle Scholar
- Gross S, Welte M, Block S, Wieschaus E: Dynein-mediated cargo transport in vivo: a switch controls travel distance. J Cell Biol. 2000, 148: 945-956. 10.1083/jcb.148.5.945.PubMed CentralView ArticlePubMedGoogle Scholar
- Gross SP, Welte MA, Block SM, Wieschaus EF: Coordination of opposite-polarity microtubule motors. J Cell Biol. 2002, 156: 715-724. 10.1083/jcb.200109047.PubMed CentralView ArticlePubMedGoogle Scholar
- Valetti C, Wetzel DM, Schrader M, Hasbani MJ, Gill SR, Kreis TE, Schroer TA: Role of dynactin in endocytic traffic: effects of dynamitin overexpression and colocalization with CLIP-170. Mol Biol Cell. 1999, 10: 4107-4120.PubMed CentralView ArticlePubMedGoogle Scholar
- Shubeita GT, Tran SL, Xu J, Vershinin M, Cermelli S, Cotton SL, Welte MA, Gross SP: Consequences of motor copy number on the intracellular transport of kinesin-1-driven lipid droplets. Cell. 2008, 135: 1098-1107. 10.1016/j.cell.2008.10.021.PubMed CentralView ArticlePubMedGoogle Scholar
- Gross SP, Guo Y, Martinez JE, Welte MA: A determinant for directionality of organelle transport in Drosophila embryos. Curr Biol. 2003, 13: 1660-1668. 10.1016/j.cub.2003.08.032.View ArticlePubMedGoogle Scholar
- Welte MA, Gross SP, Postner M, Block SM, Wieschaus EF: Developmental regulation of vesicle transport in Drosophila embryos: forces and kinetics. Cell. 1998, 92: 547-557. 10.1016/S0092-8674(00)80947-2.View ArticlePubMedGoogle Scholar
- Welte MA, Cermelli S, Griner J, Viera A, Guo Y, Kim DH, Gindhart JG, Gross SP: Regulation of lipid-droplet transport by the Perilipin homologue LSD2. Curr Biol. 2005, 15: 1266-1275. 10.1016/j.cub.2005.06.062.View ArticlePubMedGoogle Scholar
- Bickel PE, Tansey JT, Welte MA: PAT proteins, an ancient family of lipid droplet proteins that regulate cellular lipid stores. Biochim Biophys Acta. 2009, 1791: 419-440.PubMed CentralView ArticlePubMedGoogle Scholar
- Guo Y, Jangi S, Welte MA: Organelle-specific Control of Intracellular Transport: Distinctly Targeted Isoforms of the Regulator Klar. Mol Biol Cell. 2005, 16: 1406-1416. 10.1091/mbc.E04-10-0920.PubMed CentralView ArticlePubMedGoogle Scholar
- Myat MM, Andrew DJ: Epithelial tube morphology is determined by the polarized growth and delivery of apical membrane. Cell. 2002, 111: 879-891. 10.1016/S0092-8674(02)01140-6.View ArticlePubMedGoogle Scholar
- Mosley-Bishop KL, Li Q, Patterson K, Fischer JA: Molecular analysis of the klarsicht gene and its role in nuclear migration within the differentiating cells of the Drosophila eye. Curr Biol. 1999, 9: 1211-1220. 10.1016/S0960-9822(99)80501-6.View ArticlePubMedGoogle Scholar
- Fan SS, Ready DF: Glued participates in distinct microtubule-based activities in Drosophila eye development. Development. 1997, 124: 1497-1507.PubMedGoogle Scholar
- Whited JL, Cassell A, Brouillette M, Garrity PA: Dynactin is required to maintain nuclear position within postmitotic Drosophila photoreceptor neurons. Development. 2004, 131: 4677-4686. 10.1242/dev.01366.PubMed CentralView ArticlePubMedGoogle Scholar
- Fischer JA, Acosta S, Kenny A, Cater C, Robinson C, Hook J: Drosophila klarsicht has distinct subcellular localization domains for nuclear envelope and microtubule localization in the eye. Genetics. 2004, 168: 1385-1393. 10.1534/genetics.104.028662.PubMed CentralView ArticlePubMedGoogle Scholar
- Starr DA: A nuclear-envelope bridge positions nuclei and moves chromosomes. J Cell Sci. 2009, 122: 577-586. 10.1242/jcs.037622.PubMed CentralView ArticlePubMedGoogle Scholar
- Burke B, Roux KJ: Nuclei take a position: managing nuclear location. Dev Cell. 2009, 17: 587-597. 10.1016/j.devcel.2009.10.018.View ArticlePubMedGoogle Scholar
- Kracklauer MP, Banks SM, Xie X, Wu Y, Fischer JA: Drosophila klaroid encodes a SUN domain protein required for Klarsicht localization to the nuclear envelope and nuclear migration in the eye. Fly (Austin). 2007, 1: 75-85.View ArticleGoogle Scholar
- Koundakjian EJ, Cowan DM, Hardy RW, Becker AH: The Zuker collection: a resource for the analysis of autosomal gene function in Drosophila melanogaster. Genetics. 2004, 167: 203-206. 10.1534/genetics.167.1.203.PubMed CentralView ArticlePubMedGoogle Scholar
- Cooper JL, Till BJ, Henikoff S: Fly-TILL: reverse genetics using a living point mutation resource. Fly (Austin). 2008, 2: 300-302.View ArticleGoogle Scholar
- Henikoff S, Till BJ, Comai L: TILLING. Traditional mutagenesis meets functional genomics. Plant Physiol. 2004, 135: 630-636. 10.1104/pp.104.041061.PubMed CentralView ArticlePubMedGoogle Scholar
- Cooper JL, Greene EA, Till BJ, Codomo CA, Wakimoto BT, Henikoff S: Retention of induced mutations in a Drosophila reverse-genetic resource. Genetics. 2008, 180: 661-667. 10.1534/genetics.108.092437.PubMed CentralView ArticlePubMedGoogle Scholar
- Tran SL, Welte MA: In-vivo centrifugation of Drosophila embryos. J Vis Exp. 2010, pii-2005, 40Google Scholar
- Patterson K, Molofsky AB, Robinson C, Acosta S, Cater C, Fischer JA: The functions of klarsicht and nuclear lamin in developmentally regulated nuclear migrations of photoreceptor cells in the Drosophila eye. Mol Biol Cell. 2004, 15: 600-610. 10.1091/mbc.E03-06-0374.PubMed CentralView ArticlePubMedGoogle Scholar
- Beller M, Bulankina AV, Hsiao HH, Urlaub H, Jäckle H, Kühnlein RP: PERILIPIN-dependent control of lipid droplet structure and fat storage in Drosophila. Cell Metab. 2010, 12: 521-532. 10.1016/j.cmet.2010.10.001.View ArticlePubMedGoogle Scholar
- Wolins NE, Brasaemle DL, Bickel PE: A proposed model of fat packaging by exchangeable lipid droplet proteins. FEBS Lett. 2006, 580: 5484-5491. 10.1016/j.febslet.2006.08.040.View ArticlePubMedGoogle Scholar
- Sztalryd C, Xu G, Dorward H, Tansey JT, Contreras JA, Kimmel AR, Londos C: Perilipin A is essential for the translocation of hormone-sensitive lipase during lipolytic activation. J Cell Biol. 2003, 161: 1093-1103. 10.1083/jcb.200210169.PubMed CentralView ArticlePubMedGoogle Scholar
- Welte MA: Proteins under new management: lipid droplets deliver. Trends Cell Biol. 2007, 17: 363-369. 10.1016/j.tcb.2007.06.004.View ArticlePubMedGoogle Scholar
- Beller M, Riedel D, Jansch L, Dieterich G, Wehland J, Jäckle H, Kühnlein RP: Characterization of the Drosophila lipid droplet subproteome. Mol Cell Proteomics. 2006, 5: 1082-1094. 10.1074/mcp.M600011-MCP200.View ArticlePubMedGoogle Scholar
- Fauny JD, Silber J, Zider A: Drosophila Lipid Storage Droplet 2 gene (Lsd-2) is expressed and controls lipid storage in wing imaginal discs. Dev Dyn. 2005, 232: 725-732. 10.1002/dvdy.20277.View ArticlePubMedGoogle Scholar
- Teixeira L, Rabouille C, Rorth P, Ephrussi A, Vanzo NF: Drosophila Perilipin/ADRP homologue Lsd2 regulates lipid metabolism. Mech Dev. 2003, 120: 1071-1081. 10.1016/S0925-4773(03)00158-8.View ArticlePubMedGoogle Scholar
- Dworkin I, Kennerly E, Tack D, Hutchinson J, Brown J, Mahaffey J, Gibson G: Genomic consequences of background effects on scalloped mutant expressivity in the wing of Drosophila melanogaster. Genetics. 2009, 181: 1065-1076. 10.1534/genetics.108.096453.PubMed CentralView ArticlePubMedGoogle Scholar
- Zhao T, Gu T, Rice HC, McAdams KL, Roark KM, Lawson K, Gauthier SA, Reagan KL, Hewes RS: A Drosophila gain-of-function screen for candidate genes involved in steroid-dependent neuroendocrine cell remodeling. Genetics. 2008, 178: 883-901. 10.1534/genetics.107.082487.PubMed CentralView ArticlePubMedGoogle Scholar
- Harbison ST, Chang S, Kamdar KP, Mackay TF: Quantitative genomics of starvation stress resistance in Drosophila. Genome Biol. 2005, 6: R36-10.1186/gb-2005-6-4-r36.PubMed CentralView ArticlePubMedGoogle Scholar
- Myat MM, Lightfoot H, Wang P, Andrew DJ: A molecular link between FGF and Dpp signaling in branch-specific migration of the Drosophila trachea. Dev Biol. 2005, 281: 38-52. 10.1016/j.ydbio.2005.02.005.PubMed CentralView ArticlePubMedGoogle Scholar
- Kearney JB, Wheeler SR, Estes P, Parente B, Crews ST: Gene expression profiling of the developing Drosophila CNS midline cells. Dev Biol. 2004, 275: 473-492. 10.1016/j.ydbio.2004.08.047.PubMed CentralView ArticlePubMedGoogle Scholar
- Abell BM, Holbrook LA, Abenes M, Murphy DJ, Hills MJ, Moloney MM: Role of the proline knot motif in oleosin endoplasmic reticulum topology and oil body targeting. Plant Cell. 1997, 9: 1481-1493. 10.1105/tpc.9.8.1481.PubMed CentralView ArticlePubMedGoogle Scholar
- Ingelmo-Torres M, Gonzalez-Moreno E, Kassan A, Hanzal-Bayer M, Tebar F, Herms A, Grewal T, Hancock JF, Enrich C, Bosch M, Gross SP, Parton RG, Pol A: Hydrophobic and basic domains target proteins to lipid droplets. Traffic. 2009, 10: 1785-1801. 10.1111/j.1600-0854.2009.00994.x.PubMed CentralView ArticlePubMedGoogle Scholar
- Imamura M, Inoguchi T, Ikuyama S, Taniguchi S, Kobayashi K, Nakashima N, Nawata H: ADRP stimulates lipid accumulation and lipid droplet formation in murine fibroblasts. Am J Physiol Endocrinol Metab. 2002, 283: E775-783.View ArticlePubMedGoogle Scholar
- Listenberger LL, Ostermeyer-Fay AG, Goldberg EB, Brown WJ, Brown DA: Adipocyte differentiation-related protein reduces the lipid droplet association of adipose triglyceride lipase and slows triacylglycerol turnover. J Lipid Res. 2007, 48: 2751-2761. 10.1194/jlr.M700359-JLR200.View ArticlePubMedGoogle Scholar
- Ozeki S, Cheng J, Tauchi-Sato K, Hatano N, Taniguchi H, Fujimoto T: Rab18 localizes to lipid droplets and induces their close apposition to the endoplasmic reticulum-derived membrane. J Cell Sci. 2005, 118: 2601-2611. 10.1242/jcs.02401.View ArticlePubMedGoogle Scholar
- Rørth P: Gal4 in the Drosophila female germline. Mech Dev. 1998, 78: 113-118.View ArticlePubMedGoogle Scholar
- Gaspar I, Szabad J: In vivo analysis of MT-based vesicle transport by confocal reflection microscopy. Cell Motil Cytoskeleton. 2009, 66: 68-79. 10.1002/cm.20334.View ArticlePubMedGoogle Scholar
- Grönke S, Beller M, Fellert S, Ramakrishnan H, Jäckle H, Kühnlein RP: Control of Fat Storage by a Drosophila PAT Domain Protein. Curr Biol. 2003, 13: 603-606.View ArticlePubMedGoogle Scholar
- Lachaise D, David J, LeMeunier F, Tsacas L, Ashburner M: The reproductive relationships of Drosophila sechellia with D mauritiana, D. simulans, and D. melanogaster from the Afrotropical region. Evolution. 1986, 40: 262-271. 10.2307/2408806.View ArticleGoogle Scholar
- Hain D, Bettencourt B, Okamura K, Csorba T, Meyer W, Jin Z, Biggerstaff J, Siomi H, Hutvagner G, Lai E, Welte MA, Müller H-AJ: Natural variation of the amino-terminal glutamine-rich domain of Drosophila Argonaute2 is not associated with developmental defects. PLoS ONE. 2010, 5: e15264-10.1371/journal.pone.0015264.PubMed CentralView ArticlePubMedGoogle Scholar
- Wieschaus E, Nüsslein-Volhard C: Looking at embryos. Drosophila: A Practical Approach. Edited by: Roberts DB. 1998, Oxford: Oxford University Press, 179-214. 2Google Scholar
- Rothwell WF, Sullivan W: Fluorescent analysis of Drosophila embryos. Drosophila Protocols. Edited by: Sullivan W, Ashburner M, Hawley RS. 2000, Cold Spring Harbor, NY: Cold Spring Harbor Laboratory Press, 141-157.Google Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.