1. Cell Biology
  2. Developmental Biology and Stem Cells
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Microtubules provide directional information for core PCP function

  1. Maja Matis Is a corresponding author
  2. David A Russler-Germain
  3. Qie Hu
  4. Claire J Tomlin
  5. Jeffrey D Axelrod
  1. Stanford University School of Medicine, United States
  2. University of California, Berkeley, United States
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Cite as: eLife 2014;3:e02893 doi: 10.7554/eLife.02893

Abstract

Planar cell polarity (PCP) signaling controls the polarization of cells within the plane of an epithelium. Two molecular modules composed of Fat(Ft)/Dachsous(Ds)/Four-jointed(Fj) and a ‘PCP-core’ including Frizzled(Fz) and Dishevelled(Dsh) contribute to polarization of individual cells. How polarity is globally coordinated with tissue axes is unresolved. Consistent with previous results, we find that the Ft/Ds/Fj-module has an effect on a MT-cytoskeleton. Here, we provide evidence for the model that the Ft/Ds/Fj-module provides directional information to the core-module through this MT organizing function. We show Ft/Ds/Fj-dependent initial polarization of the apical MT-cytoskeleton prior to global alignment of the core-module, reveal that the anchoring of apical non-centrosomal MTs at apical junctions is polarized, observe that directional trafficking of vesicles containing Dsh depends on Ft, and demonstrate the feasibility of this model by mathematical simulation. Together, these results support the hypothesis that Ft/Ds/Fj provides a signal to orient core PCP function via MT polarization.

https://doi.org/10.7554/eLife.02893.001

eLife digest

Almost all cells exhibit some sort of polarity: the epithelial cells that line the digestive tract, for example, have an apical domain, which faces out, and a basal domain, which faces the tissue underneath. Some epithelial cells also exhibit planar cell polarity: this involves key structures within the cell being oriented along an axis within the plane of an epithelium. Disruption of planar cell polarity is associated with various developmental defects.

It is known that the planar polarity of epithelial cells relies on two molecular complexes—a ‘core’ complex and a signaling complex called the Ft/Ds/Fj system—working together. While each of these complexes contributes to whole tissues having the correct polarity, the way they interact to achieve this is not fully understood.

Now, by studying epithelial cells in the wings of fruit flies, Matis et al. have provided evidence for a specific model for this interaction. The process starts with the Ft/Ds/Fj signaling complex, which orients structures called microtubules inside the cell. Microtubules are involved in providing structural support for cells, and also in the transport of organelles within cells.

Once the microtubules are oriented in the correct direction, they help to orient the core complex by moving some of the proteins that make up this complex in a specified direction. An important future challenge will be to understand how the proteins in the Ft/Ds/Fj system interact with microtubules to give them their orientation.

https://doi.org/10.7554/eLife.02893.002

Introduction

In Drosophila and in vertebrates, six proteins constituting a ‘core’ PCP module acquire asymmetric distributions to polarize epithelial cells along a planar axis (Goodrich and Strutt, 2011). In the fly wing epithelium, three of the six proteins, Frizzled, Dishevelled and Diego (Dgo), become enriched at the distal adherens junctions (AJ), two, Van Gogh (Vang) and Prickle (Pk) localize to the proximal side, while Starry night/Flamingo (Fmi) localizes to both proximal and distal sides (Axelrod, 2009). Preferential interactions between Fmi/Fz and Fmi/Vang complexes across cell boundaries (Lawrence et al., 2004; Chen et al., 2008; Strutt and Strutt, 2008) and intercellular feedback loops (Tree et al., 2002; Amonlirdviman et al., 2005) can account for intracellular segregation of these complexes and coordinated alignment among neighboring cells. However, it remains unclear how this local polarity is globally oriented with respect to the tissue axes.

It is proposed that the Ft/Ds/Fj system, comprising the atypical cadherins Ft (Yang et al., 2002), Ds (Adler et al., 1998) and the Golgi-resident protein Fj (Zeidler et al., 1999), acts as a ‘global’ PCP module, transducing tissue level directional cues encoded by opposing Ds and Fj expression gradients, to orient the core PCP module (Yang et al., 2002; Ma et al., 2003). Though a mechanism that might transmit a directional signal from the Ft/Ds/Fj module to the core module is suggested by existing observations, important additional data are needed to support the model.

In the Drosophila pupal wing, apical non-centrosomal MTs are aligned along the proximal distal axis prior to the onset of hair growth (Fristrom and Fristrom, 1975; Eaton et al., 1996; Turner and Adler, 1998; Shimada et al., 2006). The Ft/Ds/Fj module plays an incompletely defined role in organization of these MTs (Harumoto et al., 2010), and MT-associated vesicles containing Fz are observed to preferentially move in a plus-end directed fashion toward the distal cell cortex (Shimada et al., 2006), leading to the hypothesis that Ft/Ds/Fj signals via these MTs to orient core PCP function. However, a comprehensive spatiotemporal correlation between Ds and Fj gradients, MT orientation and direction of core protein polarization has not been examined, nor have corresponding effects of global Ft/Ds/Fj perturbations on MTs and directional vesicle trafficking been examined.

In this study, we provide additional evidence for this model in the Drosophila wing. We find that the apical microtubule (MT) cytoskeleton (Eaton et al., 1996; Shimada et al., 2006; Harumoto et al., 2010) shows strong spatial and temporal correlation with core protein asymmetry throughout wing development. We show that, in the developing wing, Ds and Fj signal through a PCP-specific domain of Ft, together with one or more partially redundant, additional signal(s), to polarize these apical MTs. Ft coordinates association of MTs with apical intercellular junctions, suggesting that Ft and Ds spatially regulate capture and organization of the apical MT cytoskeleton. We show that, in addition to Fz, vesicles containing Dsh are transcytosed on these MTs, and that transcytosis is disrupted in ft or ds mutant tissue, suggesting that this trafficking provides directional bias for core protein localization. Together, our results support the hypothesis that global polarity information is provided by the Ft/Ds/Fj module and other signals to orient the apical MT network, which in turn orients polarization of the core PCP module.

Results

Spatiotemporal correlation of MT alignment and core PCP protein polarization

Apical MT alignment and orientation of core PCP protein domains have been shown to correlate, but have only been examined in several small domains during late pupal wing development (Shimada et al., 2006; Harumoto et al., 2010) (between 14 and 30 hr after puparium formation [APF]) (See also Figure 1—figure supplement 1B–D). If MT alignment provides directional bias for core protein polarization, one should observe a spatiotemporal correlation across the entire wing throughout the time core PCP proteins are polarized.

Core PCP protein polarization with respect to the tissue axes is first observed during larval wing development (Classen et al., 2005). We therefore surveyed apical MT structure beginning in third instar. To facilitate this broad analysis, we used tubulin staining. While foregoing the ability to determine plus-end orientation as provided by analysis of EB1 comets, this approach enables analysis of vastly greater numbers of MTs than does the EB1 assay, and also provides the potential to distinguish a more stable, anchored population, though in fact we see a strong correlation between results from both methods (Figure 1—figure supplement 2A–B′; Video 1). Similarly, both anti-tubulin and anti-tyrosinated tubulin antibodies produce indistinguishable results (Figure 1—figure supplement 2C).

Video 1
Live in vivo imaging of EB1::GFP and Cherry::Jupiter.

Live in vivo imaging of EB1::GFP comets and Jupiter::Cherry labeled MTs in 24 hAPF pupal wing. Refers to Figure 1—figure supplement 2.

https://doi.org/10.7554/eLife.02893.003

The earliest evident apical tubulin staining was seen in early to mid third-instar, and revealed an asymmetrical accumulation of tubulin in mostly single ‘dots’ within each cell (Figure 1A). Image analysis of the tubulin dots revealed a significant bias of dots localizing on the proximal side of the cell (side closest to the hinge fold; Figure 1—figure supplement 1A–A″). Shortly thereafter, MTs appear to fan out from these sites toward the center of the wing pounch (the future distal side) (Figure 1B). In EM images, these early MTs appear as dense bundles anchored to proximal junctions (Figure 1E).

Figure 1 with 2 supplements see all
Apical junction-anchored MTs appear in early third-instar wing discs.

(AC) Tubulin staining in progressively older third-instar wing pouch. Note the asymmetric accumulation of tubulin on the proximal side of the cell in early third-instar wing pouch and growing MTs observed in mid-late third-instar wing pouch. White arrows in the first wing disc cartoon show the proximal distal axis, with distal in the center of the wing pouch, and proximal tissue forming a ring around the future wing blade. (D) MTs in 7 hAPF pupal wing. Scale bar: 5 μm. (A′) A vertical cross-section of the early third-instar wing disc. Apical is at the top. (C′ and D′) Orientations of MTs, in the regions shown, calculated using OrientationJ, aligned with the P-D axis at each stage and location (arrows). (E) TEM micrograph of MTs in early third-instar wing pouch. Note anchored MTs at intercellular junction. (F) Schematic of organization of MTs, Ft and Ds in early third instar wing cells.

https://doi.org/10.7554/eLife.02893.004

Throughout wing development, image analysis software (‘Materials and methods’) applied to fluorescence images demonstrated that MTs are strongly aligned along the evolving P/D axis, and the orientation of MTs was reflected in the evolving pattern of polarized PCP proteins, from the radial pattern (P/D polarity vectors from hinge fold toward center of wing pouch, resulting in concentric circles of P/D cell boundaries) evident in third instar and early pupal stage (Figure 1C′–D′) to the parallel pattern of 19–30 hAPF pupal wings that presages the hair polarity pattern (Figure 1—figure supplement 1B″–D″; Strutt et al., 2002; Ma et al., 2003; Matakatsu and Blair, 2004; Classen et al., 2005; Rogulja et al., 2008; Aigouy et al., 2010; Hogan et al., 2011; Sagner et al., 2012). Importantly, at the time the MT dots appear, there is no evident core PCP protein asymmetry, whereas core PCP asymmetry becomes globally aligned along the P/D axis in slightly older discs only after apical junction-anchored MTs appear (Figure 1A–C), consistent with a requirement of the apical MT cytoskeleton for core module alignment.

It is important to note that one would not expect a perfect correlation between MT orientation and orientation of core PCP proteins. The core PCP mechanism, acting through feedback loops, is expected to optimize local alignment of core PCP proteins. This influence is stronger than the directional input produced by global directional signals, and is therefore expected produce the most locally coordinated possible alignment despite the possibility of discontinuities or irregularities in the underlying global biasing inputs (Ma et al., 2003). Nonetheless, strong correlation was seen at all times and locations examined.

Ultrastructure of apical MTs

Transmission Electron Microscopy (TEM) of 24 hr wings confirmed the previously described polarized organization of MTs that reach across the cell (Eaton et al., 1996; Shimada et al., 2006; Harumoto et al., 2010; Figure 2A), and also revealed that the previously observed associations of planar MTs with apical intercellular junctions (Fristrom and Fristrom, 1975) form juxtaposed, intercellular structures with MT anchoring sites on adjacent membranes of neighboring cells (Figure 2A,C–E). These anchoring sites were preferentially observed at P/D cell boundaries (Figure 2B). The dense, mostly single, MT organizing centers in each cell observed at the ‘dot’ stage (Figure 1E) evidently evolve into an arrangement in which multiple organizing centers are distributed around the cell in an oriented and polarized arrangement (Figure 2).

Figure 2 with 1 supplement see all
TEM micrographs showing apical MT organization in 24 hAPF pupal wings.

(A) TEM micrograph of MTs in 24 hAPF pupal wing. Note MTs anchored at both sides of intercellular junctions (arrow). (B) Graph depicting the localization of MT anchoring sites in the cell relative to the cell centroid. Plot is composed of 20 bins of 18° each. (C) Organization of the apical MT cytoskeleton traced from a single micrograph showing MTs spanning the cell preferentially in the P-D orientation. (D) TEM revealing planar MTs with anchoring sites on adjacent P-D cell membranes juxtaposed between two neighboring cells, with a sketch of the junctions and MTs. (E) Three additional images. The first is a lighter exposure of the image in D, to better reveal the structure of the junctions. Yellow arrowheads show associations of planar MTs with apical intercellular junctions. Scale bars, 100 nm. (F) TEM micrograpf showing no association of centrosome with MTs.

https://doi.org/10.7554/eLife.02893.007

We wished to determine how apical MTs are captured or nucleated at membrane junctions by staining for candidate proteins. EM images showed no association of centrosomes with MTs in non-dividing cells throughout wing development, suggesting that apical MTs are nucleated elsewhere (Figure 2F). We detected the minus-end binding proteins γ-tubulin and Patronin (Stearns and Kirschner, 1994; Goodwin and Vale, 2010) inside the cell, but not at the cell cortex, where they have been observed in other contexts (Meng et al., 2008; Feldman and Priess, 2012; Figure 2—figure supplement 1A). Consistent with this, patronin knockdown (Mummery-Widmer et al., 2009) shows no PCP phenotype. MT associated proteins β-catenin (Armadillo) (Ligon et al., 2001; McCartney et al., 2001), α-catenin (McCartney et al., 2001) and PAR-1 (Doerflinger et al., 2003; Harumoto et al., 2010) are all present symmetrically at the cell cortex but did not show asymmetric localization at the AJs, suggesting they are not involved in apical MT anchoring (Figure 1—figure supplement 1B,C). These results imply that there is an alternative mechanism that nucleates early, apical non-centrosomal MTs.

Ds and Fj gradients and Ds subcellular asymmetry align with MT orientation

What is the spatial signal that polarizes non-centrosomal MTs? Prior evidence suggests that the Ft/Ds/Fj pathway plays a role in organization of apical MTs (Harumoto et al., 2010; Marcinkevicius and Zallen, 2013). In the wing, as in other tissues, Ds and Fj are expressed in opposing gradients (Strutt et al., 2002; Ma et al., 2003; Matakatsu and Blair, 2004; Rogulja et al., 2008; Aigouy et al., 2010; Hogan et al., 2011; Sagner et al., 2012) which are converted into subcellular asymmetries of Ft and Ds heterodimers (Brittle et al., 2012). Biased subcellular orientations of asymmetric Ft-Ds heterodimers could play a role in polarization of the apical MT cytoskeleton. Consistent with this, the direction of MT growth between 14 hAPF and 30 hAPF have been shown to correlate with Ds and Fj gradient direction (Strutt et al., 2002; Ma et al., 2003; Matakatsu and Blair, 2004; Hogan et al., 2011) in the central part of the pupal wing (Harumoto et al., 2010). The possibility that the Ft/Ds/Fj system may organize apical MTs is also supported by prior EB1 comet assays showing that apical MTs are abnormal in ds mutant pupal wings, and that Ds or Ft misexpression perturbs their orientation (Harumoto et al., 2010). However, the reported assays were too limited to draw strong conclusions about overall architecture or evolution of the MT pattern (Harumoto et al., 2010).

Here, our analysis shows that MTs are generally aligned with Ds and Fj gradients from their first appearance in third instar discs (Rogulja et al., 2008), when they emerge on proximal sides of the cell cortex (Figure 1A). Throughout larval wing discs and pupal wings, MT orientation correlates with the direction of Ds and Fj gradients (Figure 1A–D, Figure 1—figure supplement 1). As noted previously (Brittle et al., 2012), in imaginal discs, when the tissue is small and gradients appear to be steeper (Figure 3—figure supplement 1C), marked subcellular asymmetry of Ft localization is observed that substantially overlaps core protein distribution (Figure 3—figure supplement 1A,B). We detect a similar relationship in pupal wings (Figure 3—figure supplements 2 and 3). The steepest regions of the gradients correspond to the most polarized MTs (compare Figure 1D to Figure 3—figure supplement 2A). Therefore, Ds and Fj gradients are appropriately aligned to polarize the MT cytoskeleton and thereby bias core PCP protein polarization from its earliest appearance. These data are consistent with the temporal requirement for Ds in the larval stage (Matakatsu and Blair, 2004; Aigouy et al., 2010).

Note that caution is required in deciphering the Ds and Fj gradients. Existing data for Fj expression all derive from Fj-LacZ expression, and should therefore be considered only approximate at best. For Ds, low magnification images can be deceptive, since excess cytoplasmic signal, in contrast to the relevant membrane pool, cannot be distinguished, and because smaller cells give the appearance of higher concentrations in low magnification even if membrane intensity is constant. Therefore, we have focused on analyzing subcellular asymmetric localization of Ds in high magnification images, and examples of these data are shown in Figure 3—figure supplements 1–4. We observe that, for the most part, asymmetry of Ds localization is very similar to that of core protein localization.

One exception is the posterior margin of the wing, where Ds often appears to be oriented more posteriorly than is Fmi, though overall levels of asymmetry are modest (Figure 3—figure supplement 4, box 5). In this region, Ds and Fmi polarities therefore appear to be less tightly coupled. While we do not know the reason for this, we can speculatively suggest several possibilities. These include (1) the tendency for the core system to promote local alignment producing a more parallel arrangement than would a direct readout of the Ds pattern; (2) that oppositely oriented Ft-Ds heterodimers are unevenly distributed despite the even distribution of total Ds; (3) the tendency of MTs to align along the long axis of the cell may be stronger than the influence of Ft-Ds. Consistent with this, MT orientation correlates more strongly with the long axis of cells than with the Ds asymmetry (Figure 3—figure supplement 4, box 5). Finally, (4) we cannot rule out the possibility that other unknown signals may also be acting on MT orientation (see ‘An independent directional signal in the wing periphery?’).

Hippo signaling-independent effects of Ft/Ds/Fj on polarity and MTs

It has been suggested that PCP defects in ds and ft mutants may be due to activation of the Hippo tumor suppressor pathway, which is also controlled by Ft/Ds/Fj, because ft mutant larval wing discs with rescued Hippo signaling show only weak PCP defects limited to the most proximal part of the wing despite the clonal PCP phenotypes observed in pupal and adult wings (Brittle et al., 2012). To better assess whether the Ft/Ds/Fj pathway modulates the MT cytoskeleton independent of Hippo signaling, and to do so across the expanse of the wing, we analyzed ftnull mutant flies rescued with FtΔECDΔN-1, a truncated form of Ft lacking a PCP signaling domain (Matakatsu and Blair, 2012). These flies are deficient for PCP signaling, but competent for Hippo pathway regulation. They showed PCP defects in the proximal-central part of the adult wing, displaying swirling patterns reminiscent of those in ft clones (Ma et al., 2003) (Figure 3A; Matakatsu and Blair, 2012). At 24 hAPF, MTs in the proximal and central part of the wing, where hair polarity is often disturbed, were randomized (Figure 3A,A′, Figure 3—figure supplement 5A,A′). In contrast, the peripheral and distal regions of these wings had more coherent hair polarity, with hairs pointing more toward the wing margin than in wildtype wings (Figure 3A), mirroring the orientation of core PCP protein domains (Figure 3—figure supplement 5A,A″). In these peripheral regions, MTs were ordered and oriented with the hairs and core PCP domains (Figure 3A″). Flies in which the Ds and Fj gradients were removed showed an essentially identical phenotype (ds38k fjN7/dsUA071 fjd1; UAS-Ds/TubP-Gal4; Figure 3—figure supplement 5B–B″). Finally, MT orientation was randomized in ft or ds clones in the same proximal part of the wing where it is disturbed in ft mutant wings rescued for Hippo signaling (Figure 3—figure supplement 5C; see also [Ma et al., 2008]). These data show that in the central part of pupal wings, MT orientation, core PCP protein polarity and adult polarity are strongly dependent on PCP signaling through Ft (Figure 3—figure supplements 5 and 6). They also suggest the existence of an additional signal, perhaps from the wing margin, that can orient MTs in the periphery of the wing.

Figure 3 with 7 supplements see all
MTs are misaligned in ft and ds mutant wing.

(AA″) Analysis of hair polarity and MT orientation in ftl(2) fd / ftGRV ActP-Gal4 UAS-FtΔECDΔN-1 mutant flies. (A′) MTs in the proximal and central part of the wing, where hair polarity is disturbed, are randomized. (A″) MTs in the distal/peripheral part of the wing are oriented with the hairs pointing toward the margin (all plots are composed of 36 bins of 5° each). (B and C) Ft-dependent instructive re-organization of the MT cytoskeleton. Wildtype cells around ft clones only see Ds in their mutant neighbors, and therefore preferentially accumulate Ft at their junction with the mutant cell. The orientation of MT dots is changed in wildtype cells around ft clones in third instar (B and B′) and 24 hr pupal wings (C and C′). White arrows show P-D axis and yellow arrowheads show MT spots initiating toward the clone rather than proximally (B′) or MTs organized perpendicular to the clone boundary (C′) rather than proximally-distally (right panels are high magnification images of left panel boxes). (C″) Orientations of MTs in the wildtype cells bordering ft clones calculated using OrientationJ. Scale bars: 50 μm (B and C) and 5 μm (B′C′). The P-D axis is defined as a radius from the center of the wing disc to the circumference, as described in Figure 1.

https://doi.org/10.7554/eLife.02893.009

Ft-Ds signaling is instructive for MT orientation

To determine whether Ft-Ds signaling regulates MT orientation in wing discs, and to determine whether it is instructive or merely necessary, we studied the boundaries of ft clones. In cells surrounding ft clones in wing discs, where unopposed Ds within the clone is expected to recruit excess Ft to the neighboring cell boundaries, nascent MT bundles are inappropriately polarized toward the cell border abutting the mutant cells (Figure 3B,B′). Similarly, in pupal wings MTs are perpendicular to the clone boundary (Figure 3C,C″), consistent with the reported non-autonomy resulting from manipulating the Ft/Ds/Fj system (Brittle et al., 2012). To quantify this result, we applied our image analysis tool to cells bordering (n = 51) ft clones in regions where MTs would otherwise be expected to run parallel to the clone border. Figure 3C″ shows that in these cells, MTs are reorganized predominantly perpendicular to the clone border. These results are consistent with the reported reversal of MT orientation in wings with an ectopic Ds gradient, although this was only examined late in the polarization process, during pupal development (Harumoto et al., 2010). Therefore, Ft and Ds are both required and instructive for MT organization.

Directed Dsh vesicle trafficking depends on Ft

Distally biased microtubule (MT)-dependent trafficking of Fz-containing vesicles has been shown to occur during polarization of the core PCP proteins, and both are sensitive to MT disruption, suggesting that transport is required for polarization (Shimada et al., 2006). Since we have proposed that Dsh is the critical determinant that must be asymmetrically localized (Amonlirdviman et al., 2005; Axelrod, 2009), we also examined Dsh::GFP vesicle movement in developing wings in the AJ plane, between 15 and 32 hr after puparium formation (hAPF). The majority of vesicles (80%, n = 1192) moved along the P/D axis, and showed a significant though modest bias towards distal vs proximal transport (Figure 4A,C–D; Video 2). Dsh::GFP vesicles exhibited two distinct patterns of trafficking. First, and most commonly, vesicles emerged from one side of the cell and were transported directly across the length of the cell to be incorporated into the membrane of an opposing cellular face (Figure 4A′; Video 2). Movement was highly linear and processive, though occasional backtracking and zig-zagging was observed. Often, multiple vesicles followed similar paths in a given cell, with vesicle scission and fusion appearing to occur repeatedly at specific sites. Second, a minority of Dsh::GFP vesicles took staggered paths without directional bias, paused frequently, and often left the apical plane of the cell (Figure 4B,B′; Video 3). The former pattern likely reflects polarized transcytosis, resulting in net transport of Dsh to the distal membrane, while the latter reflects a recycling pathway. Consistently, in fixed specimens, only a minor fraction of Dsh vesicles co-stains with the early endosome marker Rab5 or exocyst protein Sec5 (Figure 4—figure supplement 1A). Thus, a minority of vesicles moves through the recycling pathway while the majority of Dsh vesicles appears to be part of a transcytosis pathway. In contrast, we see no directionally biased trafficking of Vang::YFP vesicles (Figure 4E). Note that biased directional transport of any one component of the core PCP proteins should be sufficient to provide an input bias; bulk transport to achieve the remainder of asymmetric localization is expected to occur by diffusion in combination with feedback at intercellular junctions. Together with prior data, our observations suggest that the ‘distal’ components Fz and Dsh, but not ‘proximal’ components, are subject to directional trafficking.

Figure 4 with 1 supplement see all
Dsh::GFP vesicles move preferentially toward the distal side of the cell.

(A and B) Timelapse images of Dsh::GFP vesicles in 24 hAPF pupal wing. The majority of Dsh::GFP vesicles displayed directed, fast transcytotic movement with a distal bias (A). A minority of vesicles moved slowly along irregular paths (B) (derived from Video 2 and Video 3). (A′ and B′) Overlays of 73 frames from timelapse videos in A and B. Proximal is to the left and anterior is at the top. (C) The ratios of transcytosing Dsh::GFP vesicles at different pupal ages (n ≥ 1192). (D) Ratio of Dsh::GFP vesicles moving toward proximal, distal, anterior or posterior, or not moving (n = 50). (E) Similar plot of Vang::YFP vesicles showing absence of directed trafficking (n = 81). (F) Dsh::GFP vesicle movement inside ft clones showing little net movement and no significant bias (n = 42). (G) Dsh1::GFP vesicles in dsh1 wings showing a bias to P-D vesicle movement among vesicles showing net movement (n = 120). Numbers were too small to test significance of a possible difference between P and D. Scale bars, 5 μm. Significant differences between proximal and distal at p ≤ 0.05 using the binomial test are marked with *.

https://doi.org/10.7554/eLife.02893.017
Video 2
Live in vivo imaging of Dsh::GFP.

Live in vivo imaging of Dsh::GFP vesicles in 24 hAPF pupal wing. Refers to Figure 4A.

https://doi.org/10.7554/eLife.02893.019
Video 3
Live in vivo imaging of Dsh::GFP.

Live in vivo imaging of Dsh::GFP vesicles in 24 hAPF pupal wing. Refers to Figure 4B.

https://doi.org/10.7554/eLife.02893.020

The observed spatiotemporal organization of the MT cytoskeleton (Figure 2C) is suitable for directing biased transport of Dsh and Fz vesicles across cells (i.e., transcytosis) that could bias the direction of core PCP protein polarization. Furthermore, the repeated scission of vesicles from specific regions suggests that vesicle formation may be coupled to the locations of MT-associated junctional structures observed in EM images. Furthermore, the common directionality of these temporally clustered vesicular trafficking events suggests that individual MTs nucleated at or associated with a given junctional density, are likely to have the same polarity. Though the hypothesis that biased trafficking of Dsh and Fz depends on polarized MTs that are organized by Ft/Ds/Fj is appealing (Harumoto et al., 2010), no data directly link Ft/Ds/Fj function to directed vesicle trafficking. To test this, we examined Dsh::GFP vesicle movement in proximal ft mutant pupal wing tissue. We observed that, in comparison to wildtype cells, vesicles moved much shorter distances (or showed no net movement), without directional bias, and lacked processivity, instead taking random paths with frequent direction changes (Figure 4F).

Polarized Dsh1 vesicle trafficking is independent of core PCP polarity

Apical MTs are oriented independent of core PCP mutants fz (Shimada et al., 2006; Harumoto et al., 2010), vang (Harumoto et al., 2010) and dsh1 (Figure 4—figure supplement 1B). However, Fz vesicle trafficking was not scored in a core mutant background because vesicle production depends on most or all core proteins (Shimada et al., 2006). To verify that directed vesicle trafficking depends on Ft/Ds/Fj but not on core protein asymmetry, we measured movement of Dsh1::GFP in dsh1 flies. No core protein asymmetry is evident in dsh1 wings, but Dsh1::GFP vesicles are still produced, albeit at a lower frequency than in wildtype. We found that, unlike in ft mutant cells, most Dsh1::GFP vesicles move along the P-D axis (Figure 4G; Video 4), consistent with the presence of oriented MTs, and indicating that oriented trafficking does not depend on core protein asymmetry. We observed that Dsh1::GFP vesicles frequently fail to fuse with membranes, and compared to wildtype, more frequently disappear from the apical plane or do not exhibit overall net movement, perhaps reflecting defects specific to the Dsh1 allele. These results show that apical planar MTs that direct biased transcytosis of Dsh depend on the Ft/Ds/Fj pathway, but not on core module function. Furthermore, the movement of Dsh1 vesicles, the faster kinetics of transcytosing Dsh vesicles, and the greater processivity, compared to Fz vesicles all suggest that Dsh and Fz vesicles may be at least partially distinct populations.

Video 4
Live in vivo imaging of Dsh1::GFP in dsh1 mutant flies.

Live in vivo imaging of Dsh1::GFP vesicles in 24 hAPF dsh1 pupal wing. Refers to Figure 4G.

https://doi.org/10.7554/eLife.02893.021

Polarization is predicted to be insensitive to the shape of the Ds and Fj gradients

Our results thus far suggest that gradients of Ds and Fj expression, by producing asymmetric orientation of Ft-Ds heterodimers, provide directional information to bias core protein polarization. Given the apparent variation in asymmetry of Ft-Ds dimers at different times and places in wing development, we wished to assess the potential consequences of this variation on core PCP protein asymmetry. We therefore simulated this mechanism by adapting our previously described mathematical model for PCP signaling (Amonlirdviman et al., 2005; Ma et al., 2008). The modified model establishes a MT network with polarity determined by the relative concentrations of Ft on any side of a cell. User-defined input gradients of Ds and Fj determine Ft concentrations in a manner consistent with the experimentally defined model. Dsh is then transported toward the plus ends of MTs, while still permitting bulk movement of all components by diffusion (see Supplementary file 1). We first validated the model by correctly reproducing the domineering non-autonomy (or lack thereof) surrounding clones of core PCP mutants (Figure 5—figure supplement 1). Furthermore, we confirmed that the model correctly simulates the ability of the core module to propagate polarization across small ft mutant clones (Figure 5—figure supplement 1).

The model then allowed us to predict the response to different configurations of the Ds or Fj gradients. As discussed above, there is considerable ambiguity about the shape of the Ds gradient through wing development, but to a first approximation, it appears to undergo considerable change from larval wing discs, where there is a comparatively linear gradient, at least in the distal portion of the wing not hidden by tissue folds, to one with a steep drop and very shallow or flat portion in the 24–30 hr pupal wing (Figure 3—figure supplements 1–4; Ma et al., 2003; Matakatsu and Blair, 2004; Hogan et al., 2011). In third instar discs, gradients of Ds and Fj are roughly linear (Figure 3—figure supplement 1C). In simulation, oppositely oriented linear gradients of Ds and Fj polarize a field of cells with similar kinetics and identical steady state levels of polarization across the entire field. Whereas in the larval wing disc, the Ds gradient may be gradual, in the pupal wing, the gradient of Ds approaches a step gradient as it rearranges first to a projection of high Ds in the central part of the pupal wing, and later to a very high proximal concentrations and a shallow or even flat distal distribution. Notably, simulation of a linear gradient, a step gradient, or a steep proximal Ds gradient and a shallow or flat distal gradient produces identical levels of steady state polarization across the field and similar proximal and distal kinetics, showing that the mechanism is not expected to be very sensitive to the precise shape of the Ds gradient (Figure 5). In the cases of a steep local Ds gradient, propagation of Ft-Ds polarity into an adjacent shallow or flat region is weak, and limited to two columns of cells (data not shown), most likely due to absence of a robust feedback mechanism in our model. Similarly, propagation of Ft-Ds polarization in vivo is seen to be much weaker than that of the core PCP mechanism (c.f. Ambegaonkar et al., 2012; Brittle et al., 2012). Therefore, propagation of polarity through the shallow or flat region is primarily due to polarization and propagation of the core PCP system.

Figure 5 with 1 supplement see all
Simulations of polarization kinetics with different shapes of Ds gradients or imposed MT structures, using a mathematical model incorporating a simple representation of the Ft/Ds/Fj system to polarize MTs.

Input Ds gradients are shown on the left. Resulting (or imposed, on the right side of the last example) MT organization on the proximal or distal portion of the gradient are plotted (center). Kinetics of polarization of cells in column 8 (proximal = left), column 15 (center) or column 23 (distal = right; see Figure 5—figure supplement 1).

https://doi.org/10.7554/eLife.02893.022

In the distal part of the wing, MTs are oriented in the P-D direction, but have no detectable polarity bias. We therefore simulated several additional conditions. First, we simulated a steep proximal gradient with a distal zero level of Ds that produces randomized distal MT orientation in our model. Global directional input is therefore restricted to the proximal region. In this case, we see equivalent proximal and distal steady state polarization, but with a substantial delay in reaching steady state in the distal region, reflecting time needed to propagate polarity from proximal to distal through the core mechanism. To simulate MTs that are P-D oriented, but without a measurable plus-end bias, as are observed in pupal wings, we enforced this MT architecture in the distal wing, with a steep proximal Ds gradient. Simulation of this condition predicts modestly faster core PCP polarization compared to random distal MTs, but not to change steady state core PCP polarization. Therefore, the observed unbiased but oriented MTs in the distal wing might facilitate more rapid core PCP polarization and also maintenance of polarity in the face of perturbations.

In similar simulations, we tested the response to different configurations of the Fj gradient. Again, we found that steady state polarization is insensitive to the gradient configuration, with only slight differences in kinetics (data not shown). A similar result was obtained when simultaneously altering the shapes of both gradients (data not shown). From these simulations, we conclude that so long as the Ds and Fj gradients are in the proper direction, their potentially evolving profiles are not expected to have a substantial effect on the resulting core PCP polarity.

An independent directional signal in the wing periphery?

Distal (peripheral) polarity is independent of Ft function; polarity in this region may depend on a spatial signal perhaps originating from the wing margin. A candidate for this signal is the proposed redundant functions of Wnt4 and Wg. Both are expressed at the wing margin, combined loss-of-function produces a mild polarity phenotype, and overexpression of Wnt4 to a much greater extent than Wg perturbs hair polarity (Lawrence et al., 2002; Lim et al., 2005; Wu et al., 2013). Based on a cell culture assay, these Wnts were suggested to impact core PCP function by blocking interactions between Fz and Vang. However, our observation that a Ft independent signal might polarize MTs near the wing margin suggests that other possible mechanisms should be considered. Notably Wnt4 (but not Wg) overexpression reorganizes MTs (Figure 3—figure supplement 7), suggesting that a different possible mechanism for Wnt4 function should be entertained.

Discussion

Together, our findings support the hypothesis that a polarized MT cytoskeleton orients PCP throughout wing development by directing the trafficking of Dsh containing vesicles. Furthermore, they confirm that the Ft/Ds/Fj PCP module directs orientation of this apical MT cytoskeleton, at least in the proximal central portion of the wing.

We infer that a second signal, acting near the wing margin and perhaps originating from the margin, can also organize MTs to orient the core PCP mechanism. The recent finding that Wnts expressed at the wing margin regulate PCP suggests a possible identity for this signal (Wu et al., 2013). We propose that in third instar wings, when the tissue is smaller, the two signals are largely redundant, so that defects in Hippo-rescued ft mutants are limited to the most proximal regions (Feng and Irvine, 2007; Brittle et al., 2012; Matakatsu and Blair, 2012; Pan et al., 2013), whereas in larger pupal and adult wings, Hippo-rescued ft mutants show larger regions of disturbed polarity. One difficulty in understanding how a wing margin-based signal might contribute to polarization is that much of the anterior and posterior margin is parallel to the direction of polarization, while the distal portion of the margin is perpendicular. Additional studies will be needed to understand potential signals from the margin.

Notably, even in regions well polarized by the presumed wing margin signal, ectopic Ds expression can reorganize polarity (Matakatsu and Blair, 2004; Harumoto et al., 2010). Furthermore, the strong correspondence of MT orientation and core protein orientation throughout wing morphogenesis, their overall correspondence to Ds-Fj gradients, and the ability of altered Ft or Ds expression patterns to reconfigure MT orientation, suggest that these gradients provide instructional information for core PCP orientation, at least in the proximal and central region of the wing. This signal likely acts in conjunction with other molecular signals, particularly in the peripheral region of the wing, and perhaps with mechanical inputs such as cell flow and cell elongation (Aigouy et al., 2010).

Recently, it was shown that the tissue and compartment specific expression predominance of the Pk vs Spiny-legs isoforms of Pk determines the direction of Ds and Fj gradient interpretation (Ayukawa et al., 2014; Olofsson and Axelrod, 2014). Thus, for example, polarization of the core module can occur in the same direction in the Anterior and Posterior compartments of the abdomen despite oppositely oriented Ds and Fj gradients in these compartments.

In summary, we provide evidence favoring the model that the Ft/Ds/Fj global PCP module, together with a partially redundant and as yet unidentified peripheral wing signal, orients apical polarized microtubules, directing Dsh-vesicle transcytosis, and thereby imparting directional information to the core PCP module. To what extent other global signals may function in other tissues remains to be determined. The presence of polarized MTs suggests that a MT dependent global cue may also function in vertebrate PCP (Vladar et al., 2012).

Materials and methods

Drosophila stocks

The following fly lines and mutant alleles were used:

  • OreR,

  • Dsh::GFP,

  • actinP-Vang::EYFP,

  • Ds::GFP (Brittle et al., 2012),

  • ciGal4/UAS-EB1::GFP,

  • ubi-Jupiter::mCherry,

  • armP-Fz::GFP,

  • ftl(2) fd FRT40A Dsh::GFP/NLS::mRFP FRT40A; T155Gal4 UAS-FLP/+,

  • ftGRV FRT40A,

  • ftGRV FRT40A/ftl(2) fd FRT40A; UAS-FtΔECDΔN1 (Matakatsu and Blair, 2012)/ActP-Gal4,

  • ds38k fjN7/dsUA071 fjd1; UAS-Ds/TubP-Gal4,

  • hs-FLP; dsUA071 FRT40A/FRT40A Tub-Gal80; TubP-Gal4 UAS-mCD8GFP/+,

  • ftGr-V FRT40A/FRT40A Tub-Gal80; TubP-Gal4 UAS-mCD8GFP/+,

  • ftl(2)fd dGC13/ftl(2)fd d1,

  • enGal4/UAS-Wnt4.

Immunohistochemistry

Drosophila pupal wings were prepared for imaging as previously described (Axelrod, 2001). Primary antibodies were as follows: mouse anti-Fmi (#74, Developmental Studies Hybridoma Bank), mouse anti-Arm (Developmental Studies Hybridoma Bank), rabbit anti-alpha Tubulin (Abcam, Cambridge, UK), rat anti-tyrosinated Tubulin (Abcam, Cambridge, UK), rat anti-Ds and rat anti-Ft (Yang et al., 2002). Images were acquired on a Leica TCS SP5 AOBS confocal microscope using a 63x objective and processed with LAS AF (Leica).

TEM

For EM analysis, wing imaginal discs and pupal wings were fixed in a mixture of 4% paraformaldehyde and 2% glutaraldehyde in 0.1 M sodium cacodylate buffer, pH 7.3 overnight at RT. Samples were post-fixed in 1% osmium tetroxide in 0.1 M PBS for 1 hr at RT, stained with uranyl acetate, dehydrated with a graded ethanol series and embedded in EMbed-812 (Electron Microscopy Sciences). Ultrathin sections were cut and analyzed with a JEOL JEM-1400 microscope using a Gatan Orius Camera.

Time-lapse imaging

For live imaging, pupae were removed from incubation at 25°C 10 min prior to the desired time APF. Pupae were mounted on a small piece of double-sided tape and forceps were used to dissect open a small window in their pupal cases to provide visual access to the live pupal wing. Approximately 50 μl of halocarbon oil was placed over each dissected pupa to allow its release from the tape, following which the pupae were mounted on a VivaScience petriPERM 50 hydrophobic membrane disk in halocarbon oil between pieces of hydrated Whatman paper for in vivo confocal fluorescence microscopy. Videos showing Dsh::GFP and membrane RFP (used to mark wildtype cells) show that internalized Dsh::GFP is always seen to co-stain with RFP. Furthermore, Shimada et al. reported that in fixed images the majority of Dsh and Fz vesicles overlap (Shimada et al., 2006). We are therefore confident that internalized Dsh::GFP is in vesicles.

Image analysis

For analysis of MT orientation we used OrientationJ software (Rezakhaniha et al., 2012). We analyzed an average of 20 images from 5 to 10 wing discs or pupal wings for each time point or genotype. The images were taken from appropriate parts of the wing as shown in figures and aligned along the P/D axis (which is plotted as horizontal) of the wing disc or pupal wing.

Analysis of MT anchoring sites in 24 hAPF wings was done using ImageJ.

To analyze the localization of apical tubulin in early third-instar wing pouch we used the cross correlation method as previously described (Matis et al., 2012).

For analysis of live imaging time-series, vesicles were only measured and quantified if they were visible in two or more consecutive frames at the level of the adherens junctions. Images were taken at 5 s intervals. We analyzed manually 1192 particle tracks to calculate the net direction of movement (proximal, distal, anterior, posterior or ‘stuck’–no change in location between any two consecutive frames). A vector was taken between the first and last points of each track to calculate the net direction of movement.

Mathematical modeling

A mathematical model, incorporating the proposed mechanism of the Ft/Ds/Fj module to organize MTs, has been created based upon our previously published ODE model (Ma et al., 2008). Details are described in Supplementary file 1. Simulations of clones (Figure 5—figure supplement 1) or of wildtype grids with user defined Fj and Ds gradients (Figure 5) were performed to assess kinetics and quasi-steady state levels of polarization.

References

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Decision letter

  1. Helen McNeill
    Reviewing Editor; The Samuel Lunenfeld Research Institute, Canada

eLife posts the editorial decision letter and author response on a selection of the published articles (subject to the approval of the authors). An edited version of the letter sent to the authors after peer review is shown, indicating the substantive concerns or comments; minor concerns are not usually shown. Reviewers have the opportunity to discuss the decision before the letter is sent (see review process). Similarly, the author response typically shows only responses to the major concerns raised by the reviewers.

Thank you for sending your work entitled “Initiation and evolution of asymmetric microtubules by Ft/Ds/Fj in planar polarization of Drosophila wing epithelium” for consideration at eLife. Your article has been favorably evaluated by K VijayRaghavan (Senior editor) and 4 reviewers, one of whom is a member of our Board of Reviewing Editors.

The Reviewing editor and the other reviewers discussed their comments before we reached this decision, and the Reviewing editor has assembled the following comments to help you prepare a revised submission.

All the reviewers thought there is value in the manuscript, that it adds to the ongoing discussion of the placement of the Ft/Ds and core PCP pathway, and contributes information to the state of microtubules during the development of polarity. However there were 4 major areas that all the reviewers agreed needed to be addressed/improved before this manuscript would be acceptable at eLife. In addition there were issues where the figure needed improvement, and the text could benefit from clarification. These points are detailed below.

1) The modeling in its present state does not add substantially to the paper

Reviewer 1: “The authors need to explain some basics about how their model works in the text. How is the Fat-Ds-MT connection modeled? How is it tied to the core proteins? Is there a mechanism for core polarization independent of the MT orientation? As is, the authors state nothing, except for equations buried deep in a supplement.

Then, there is the question of what the model shows, beyond what is intuitively obvious. What the authors claim is oddly spotty. The model is based on a published model that already had the ability to predict autonomy or non-autonomy of the core mutant clones, even without including anything about Fat-Ds-MTs. So the fact that it still does so, the first statement the authors make about the model, is not very surprising.

The old model also showed non-autonomy, so the fact that the new model can show non-autonomy through small fat mutant clones only means that the inclusion of the Fat-Ds-MT equations has not changed much.

The only effect of the new equations that the authors show is that changing between various Ds gradients can change the kinetics of core protein polarization. But they do not even mention the effect of flat Ds expression, or missing Fat. Does it reproduce the effects of missing ds and fj, or uniform ds and fj?

They only show effects on the core proteins. Does the model correctly predict known effects on propagation of Ds-Fat polarization? Does it predict the non-autonomous effects of fat clones on MT orientation?

Reviewer 2: “the model shows how altered Ds gradients might affect MT orientation and Core protein migration. In contrast, the manuscript does not describe experiments in which Ft/Ds gradients alter MT orientation and so determine the direction of Core protein migration. Altered ft/ds activity, MT polarity, PCP protein accumulation and hair polarity”

Reviewer 3: “One of the values of the modelling is that it enabled the authors to test the effects, if any, of alternative Ds gradients. However, none of the alternatives tested resembled the Ds distributions shown in Figure 3–figure supplement 2. I would really like to see those tested.”

2) The manuscript needs more extensive quantification and characterization of the MT changes

Reviewer 2: “The most significant finding described in the manuscript (in my opinion) is the ability of altered Ft/Ds activity to be 'instructive' for MT orientation. This is shown in cells surrounding ft loss of function clones. However, in terms of quantification, this is, perhaps, the weakest part of the manuscript. Two clones are shown with just a few cells indicated to show altered MT orientation (Figure 3B,C). The authors made a lot of clones (Figure 3B) so a more quantitative analysis of cell non-autonomy could have been undertaken. Also, they might discuss these cell non-autonomous changes in MT orientation with respect to the cell non-autonomous effects of ft clones on wing hair polarity. It seems (to me) that in cells with altered MT orientation (Figure 3C'), the Core protein Fmi (green) is also localized perpendicular to the clone. I would expect Fz/Dsh to localize with Fmi at one end of the cell. Therefore, it does not appear that Fz/Dsh migration along the reoriented MTs is determining Core protein localization. The authors should discuss this.

“The authors describe a 'strong correlation' between the tubulin staining (presented) which defines MT orientation, and EB1 assay data (not presented), which can show both MT orientation and polarity. Since MT polarity may instruct Core protein migration, it would be useful to see the authors' EB1 data.”

Reviewer 3: “Tyr-tubulin primarily detects very dynamic microtubules. Did the authors see the same bias when using general anti-Tubulin antibodies? If this was stated I did not see it. Given that the microtubule bias they detect is long lasting I am surprised at the antibody choice.”

In the Results section the authors state “…asymmetrical accumulation of tubulin in single “dots” within each cell (Figure 1A)”. There are certainly dots that are asymmetric but a substantial minority of the cells have more than one dot. This should be quantitated.

Reviewer 1: “The authors state that “Throughout larval wing discs and pupal wings, MT orientation correlates with the direction of Ds and Fj gradients”. However, at later pupal stages there is a stripe of strong Ds expression that extends into the central portion of the wing blade, which adds a considerable anterior/posterior bias to the Ds gradient in non-central regions of the wing, and which is obvious in the author's photo at 24 hours. Published evidence suggests that this anterior-posterior gradient is instructional for PCP, at least in some mutant backgrounds. Yet the core proteins do not orient along this gradient after their 16 hour reorientation, as noted by the Eaton lab, and from the authors' figures of 24 hour wings the MTs follow the core proteins, not the Ft-Ds-Fj gradient, in non-central regions.

Thus, the correlation is likely less global than the authors state, at least at later stages and non-central regions. If so, the authors are oversimplifying. The pertinent figure, Figure 3–figure supplement 1C“, shows details of what I suspect are the central region of the wing at 24 hours AP. If the authors have non-central figures that support a global correlation at all stages and locations, they should show them. If not, they need to modify their statements.”

“Disruption of MT organization in the ds mutant was incomplete, displaying unexpected underlying structure, and the altered directionality upon misexpression was not consistent with a simple redirection of MT orientation.”

This is a very interesting result, but the authors should show it. It is also worth a brief discussion, as it differs from the effects of ds fj. How is Fj functioning in a ds mutant, where Ft-Ds binding is lost?

Similarly, in pupal wings MTs are perpendicular to the clone boundary (Figure 3C,C'),” I had difficulty seeing this, especially given the variable orientation elsewhere. This would be much more convincing if the authors could quantify it.

3) Clarification of the Ds gradient

Reviewer 1: “the Ds gradient undergoes considerable change from a relatively linear gradient earlier to one with a steep drop and very shallow or flat portion in the 24-30 hour pupal wing (Figure 3–figure supplement 1C' and ref. (Matakatsu and Blair, 2004, Hogan et al., 2011a, Ma et al., 2003)” and “In the larval wing disc, the Ds gradient is gradual, while in the pupal wing, the gradient of Ds approaches a step gradient as it rearranges first to a projection of high Ds in the central part of the pupal wing, and later to a very high proximal concentrations and a shallow or even flat distal distribution.”

Firstly, it is not clear which of several stages the authors are referring to by “pupal” or “earlier”. Secondly, is the disc gradient really more gradual? The authors do not show a picture, and I do not remember anything convincing from the literature, especially because the proximal half of the wing blade is hiding in a fold at late third. If the authors could show a good picture, that would be valuable, but it would have to include a cross-section to show the tissue in the fold.

The early pupal wing picture in Matakatsu does look very abrupt, with very high Ds near the hinge, but confusingly Figure 3–figure supplement 1C (7 hours) does not look like a step because it cuts off the proximal wing with the highest Ds levels. 1C” (24 hours) looks pretty abrupt proximally, but there looks to be a gradual gradient along the bit that extends out between the central veins.

While the authors make abruptness of the Ds gradient shape a major point of their model, they ignore the modifying effect of the Fj gradient. And the scale of the model is also quite short (only 30 cells) compared with the actual wing blade, so it is not clear how biologically relevant this is.

Finally, what Ds pattern or data does “In comparison to MTs in the distal region, simulation of an unbiased but oriented arrangement is predicted to modestly speed polarization compared to random MTs, but not to change steady state polarization” refer to?

4) Questions on the relevance of the Wnt gradient discussion

Reviewer 2: The authors suggest a second signal from the margin orients microtubules in the non-proximal, central part of the wing and suggest this could be due to Wnts. That is a reasonable suggestion however the paper referenced that showed margin Wnts played a role in PCP made the argument it did this by modulating core protein activity. However, the literature argues the core proteins do not play a role in MT orientation. Are the authors suggesting that margin Wnts have two functions - one to orient MTs and a second to modulate core proteins? Do they think the previous papers missed a disruption of MT orientation in core mutants in the distal region? Of course in a fz or dsh mutant wing the polarity of hairs is only slightly altered in the most distal part of the wing so other factors are likely important.

Reviewer 1: “They also suggest the existence of an additional signal from the wing margin that can orient MTs” and “Distal (peripheral) polarity is independent of Ft function, but appears to depend on a Wnt-dependent signal from the wing margin (Wu et al., 2013) that one can speculate might orient but not bias MTs.”

First, the authors have no evidence for the source of the missing signals. Second, even if they are wing margin Wnts, there is no evidence that this can control MT polarity. Instead, the quoted work suggests a fairly direct interaction between Wnts and core protein activity, and there is no evidence that changing core protein activity can orient MTs. I think the comments should take this into account. Or the authors could test this by overexpressing Wnt4 and looking.

Reviewer 3: It seems unlikely that Wnt is functioning with Core proteins in a 'non-canonical' pathway as well as acting upstream to control MT orientation.

https://doi.org/10.7554/eLife.02893.025

Author response

1) The modeling in its present state does not add substantially to the paper

We regret that our goal for the modeling was not well articulated, and the revision explains this more clearly. The intent was solely to investigate how changes in the profile of the Ds gradient (in other words, the steepness as a function of distance) along an axis, affect the kinetics of polarization and the steady state polarity. We conclude that differences in the profile have no effect on steady state, and in most cases only subtle effects on the kinetics. This is important, as it seems that the gradients evolve over time, and one might wonder if this has any consequence. We have now extended this result to Fj, with essentially similar results.

We have not attempted to model the radial patterns (a very different question, but we believe this would be a rather uninformative exercise). It would clearly be possible to achieve such a pattern in simulation, but it is not apparent to us what we would learn.

2) The manuscript needs more extensive quantification and characterization of the MT changes

Reviewer 2: “The most significant finding described in the manuscript (in my opinion) is the ability of altered Ft/Ds activity to be 'instructive' for MT orientation. This is shown in cells surrounding ft loss of function clones. However, in terms of quantification, this is, perhaps, the weakest part of the manuscript. Two clones are shown with just a few cells indicated to show altered MT orientation (Figure 3B,C). The authors made a lot of clones (Figure 3B) so a more quantitative analysis of cell non-autonomy could have been undertaken. Also, they might discuss these cell non-autonomous changes in MT orientation with respect to the cell non-autonomous effects of ft clones on wing hair polarity. It seems (to me) that in cells with altered MT orientation (Figure 3C'), the Core protein Fmi (green) is also localized perpendicular to the clone. I would expect Fz/Dsh to localize with Fmi at one end of the cell. Therefore, it does not appear that Fz/Dsh migration along the reoriented MTs is determining Core protein localization. The authors should discuss this.

We agree with the reviewer that quantification of MT polarity around Ft clones is warranted. We have now quantified MT orientation around clones and included aggregated results in the new graph in Figure 3. To do this, we analyzed anterior and posterior clone borders, where MTs would normally run parallel to the border. As is evident from the added graph in Figure 3C’’, a majority of MTs is reoriented to run orthogonal to the border.

The reviewer raises a complex question about the cell non-autonomous effects of ft clones on hair polarity. It is indeed correct that some ft clones, primarily larger ones, or those that traverse regions with more irregular cell geometry, such as veins, are more likely to produce swirling hair polarity patterns. This was analyzed previously in Ma et al PNAS 2008. In these cases, Fmi and other core proteins are mislocalized in concordance with the hair polarity pattern. The reviewer wonders why MTs might be oriented differently from the core protein pattern at clone boundaries. Perhaps the simplest case is the one in which a modest sized ft clone does not alter core protein or hair polarity. Here, MTs are still misoriented next to the clone (at A-P oriented edges). To explain this, one must keep in mind that while our hypothesis is that the polarity of a cell is biased by the orientation of MTs, a stronger influence is the tendency of core function to locally align polarity between cells (see Ma et al 2003 for discussion of this phenomenon). To minimize discontinuities in local polarity, this influence will override the influence of the global Ft dependent signal via MTs. A system with this design will produce highly coordinated polarity even in the presence of an imprecise global signal resulting from imprecise gradients, as must necessarily be generated over such a long range.

If the editors believe it would be beneficial, we can include more extensive discussion of this point in the text, but since its essence has already been published and discussed, we feel it would be distracting to the flow of the logic.

“The authors describe a 'strong correlation' between the tubulin staining (presented) which defines MT orientation, and EB1 assay data (not presented), which can show both MT orientation and polarity. Since MT polarity may instruct Core protein migration, it would be useful to see the authors' EB1 data.”

A figure and movie of pupal wing co-expressing EB1::GFP and Jupiter::Cherry were added (Figure 1–figure supplement 2).

Reviewer 3: “Tyr-tubulin primarily detects very dynamic microtubules. Did the authors see the same bias when using general anti-Tubulin antibodies? If this was stated I did not see it. Given that the microtubule bias they detect is long lasting I am surprised at the antibody choice.

We obtained the same result with both Abs, anti-Tyr Tubulin and anti-alpha Tubulin (Figure 1–figure supplement 2C).

In the Results section the authors state “…asymmetrical accumulation of tubulin in single “dots” within each cell (Figure 1A).” There are certainly dots that are asymmetric but a substantial minority of the cells have more than one dot. This should be quantitated.

Indeed, a minority of cells has more than one ‘dot’. We speculate that these represent the beginning of the eventual distribution of MT anchoring sites around the cell periphery, though this would be extremely challenging to prove. Furthermore, in cells that are dividing, anti-tubulin Ab also labels the two spindles/centrosomes, and thus in some cases two dots may indicate dividing cells. We have not quantified this, as the number would not have any clear significance.

Reviewer 1: “The authors state that “Throughout larval wing discs and pupal wings, MT orientation correlates with the direction of Ds and Fj gradients”. However, at later pupal stages there is a stripe of strong Ds expression that extends into the central portion of the wing blade, which adds a considerable anterior/posterior bias to the Ds gradient in non-central regions of the wing, and which is obvious in the author's photo at 24 hours. Published evidence suggests that this anterior-posterior gradient is instructional for PCP, at least in some mutant backgrounds. Yet the core proteins do not orient along this gradient after their 16 hour reorientation, as noted by the Eaton lab, and from the authors' figures of 24 hour wings the MTs follow the core proteins, not the Ft-Ds-Fj gradient, in non-central regions.

In early pupal wings (7 hAPF), the Ds gradient is radial, but gradually evolves into a more linear organization. We agree with the reviewer that there is still a detectable stripe of Ds expression near the proximal part of the L3 vein at 24 hours, but careful examination reveals that this impression, gleaned from lower magnification images, reflects higher cytosolic concentrations of Ds and also perhaps the small cells that comprise the vein. In contrast, membrane bound Ds, the relevant population, is polarized perpendicular to this Ds gradient along the P/D axis by 24 h APF. We now include additional images showing asymmetry of membrane associated Ds along the P/D axis in this region of the wing (Figure 3–figure supplement 4).

Thus, the correlation is likely less global than the authors state, at least at later stages and non-central regions. If so, the authors are oversimplifying. The pertinent figure, Figure 3–figure supplement 1C“, shows details of what I suspect are the central region of the wing at 24 hours AP. If the authors have non-central figures that support a global correlation at all stages and locations, they should show them. If not, they need to modify their statements.

We now include additional images of the whole wing showing Ds and core polarity at 26APF, as well as higher magnification images from selected regions. However, in a different context, the reviewer is correct: We point out that there is a possible discrepancy in the orientation of Ds with respect to core protein orientation in the posterior region of the wing, near the posterior margin. In this region, the core proteins appear to be oriented with a mostly proximal-distal polarity, whereas the Ds stain appears to be oriented with a somewhat A-P polarity. While this potential discrepancy may be enhanced by ‘illusion’ due to the relatively elongated cell shapes and cell packing organization that is observed in this region, we think there is indeed some difference in direction in this region. In high magnification images (some more than others), there is modest evident enrichment of Ds in a more posterior orientation. We do not have a solid explanation, but now discuss several possibilities in the text. It is important to note that this is a region of the wing where the Ft/Ds/Fj module is less important, or at least perhaps redundant with another signal.

“Disruption of MT organization in the ds mutant was incomplete, displaying unexpected underlying structure, and the altered directionality upon misexpression was not consistent with a simple redirection of MT orientation.

This is a very interesting result, but the authors should show it. It is also worth a brief discussion, as it differs from the effects of ds fj.

The first part of this sentence is meant to refer to results in Harumoto (2010), where in the distal part of the wing, MTs are P-D without much or any bias in polarity in wild type, but in the ds mutant, show a modest plus end proximal polarity. We have no good explanation for this, but it may be related to the observation that Ft clearly has some influence in the absence of Ds, or perhaps to other influences that are unmasked by loss of Ds. The second part refers to a complex experiment in which MT polarity was measured across the boundary of en-GAL4 UAS-Ds expression, and gave a confusing result. Both of these allusions were unnecessarily oblique, and have been deleted.

We don’t think there’s an important difference between the Harumoto ds loss of function result and our Ds Fj analysis, as these statements refer to different locations. Their result to which we refer was near the distal end of the wing; they also show loss of organization proximally.

Similarly, our results show loss of parallel organization in the proximal/central part of the wing but not distally (with some other signal presumably organizing the distal region, as discussed in this manuscript and below).

How is Fj functioning in a ds mutant, where Ft-Ds binding is lost?

Again, we don’t know, but may be related to the Ds independent function of Ft, which is also a substrate for Fj. This is an interesting and important question that is well beyond the scope of this manuscript.

Similarly, in pupal wings MTs are perpendicular to the clone boundary (Figure 3C,C'),” I had difficulty seeing this, especially given the variable orientation elsewhere. This would be much more convincing if the authors could quantify it.

As discussed above, this is now quantified.

3) Clarification of the Ds gradient

Reviewer 1: “the Ds gradient undergoes considerable change from a relatively linear gradient earlier to one with a steep drop and very shallow or flat portion in the 24-30 hour pupal wing (Figure 3–figure supplement 1C' and ref. (Matakatsu and Blair, 2004, Hogan et al., 2011a, Ma et al., 2003)” and “In the larval wing disc, the Ds gradient is gradual, while in the pupal wing, the gradient of Ds approaches a step gradient as it rearranges first to a projection of high Ds in the central part of the pupal wing, and later to a very high proximal concentrations and a shallow or even flat distal distribution.

Firstly, it is not clear which of several stages the authors are referring to by “pupal” or “earlier”.

Corrected – Figures of several stages have been added as supplements to Figure 3. We have tried to clarify the language used to describe these observations.

Secondly, is the disc gradient really more gradual? The authors do not show a picture, and I do not remember anything convincing from the literature, especially because the proximal half of the wing blade is hiding in a fold at late third. If the authors could show a good picture, that would be valuable, but it would have to include a cross-section to show the tissue in the fold.

We have added an image showing this, at least for the distal part of the wing blade that is not hidden in the fold (Figure3–figure supplement 1C).

The early pupal wing picture in Matakatsu does look very abrupt, with very high Ds near the hinge, but confusingly Figure 3–figure supplement 1C (7 hours) does not look like a step because it cuts off the proximal wing with the highest Ds levels.

While our image of a 7 hour wing does not show all of the hinge, it was visualized by Matakatsu, (although with LacZ, so that staining may reflect earlier expression).

1C“ (24 hours) looks pretty abrupt proximally, but there looks to be a gradual gradient along the bit that extends out between the central veins.

Indeed, the gradient appears to be steep at 24 hours, with a shallower portion extending into the blade. However, as discussed above, and now in the text as well, all of these observations from low magnification images should be taken with a grain of salt, as they do not distinguish membrane from cytoplasmic/internal protein, nor can they distinguish true differences in amount from variation in cell size (smaller cells give the appearance of higher concentrations at low mag). To address all of these concerns, we have added some explanation to the text, and pointed out the important take home message, which is that the true steepness of the gradient of membrane associated Ds is ambiguous and might change over time. This should be distinguished from the direction of Ds asymmetry, which can be clearly read from high magnification images.

As a final note to this point, there is now evidence that non-autonomy and local feedback within the Ft-Ds mechanism that would be expected to locally align the polarity of these molecules, perhaps overriding the effects of reading gradients alone.

While the authors make abruptness of the Ds gradient shape a major point of their model, they ignore the modifying effect of the Fj gradient. And the scale of the model is also quite short (only 30 cells) compared with the actual wing blade, so it is not clear how biologically relevant this is.

We chose to address only the Ds gradient because this is the one for which there is any real data. Because of the lack of a Fj antibody that works for immunofluorescence, there are only LacZ data for Fj, and perdurance makes these unreliable for addressing changes with time. We therefore left the Fj gradient constant. However, we have now done similar simulations for Fj, and find essentially similar results. This is now noted in the text.

Finally, what Ds pattern or data does “In comparison to MTs in the distal region, simulation of an unbiased but oriented arrangement is predicted to modestly speed polarization compared to random MTs, but not to change steady state polarization” refer to?

This experiment is meant to test the potential relevance of proximally-distally oriented but unbiased MTs that is actually observed in the distal part of the wing as reported by Harumoto et al 2010. The result is a modest increase in the rate of polarization, but equivalent steady state.

This is part of the larger question, much debated in our lab, about the relevance of these MTs in the distal part of the wing. The language in the manuscript has been clarified.

4) Questions on the relevance of the Wnt gradient discussion

[…] Reviewer 1: “They also suggest the existence of an additional signal from the wing margin that can orient MTs” and “Distal (peripheral) polarity is independent of Ft function, but appears to depend on a Wnt-dependent signal from the wing margin (Wu et al., 2013) that one can speculate might orient but not bias MTs.

First, the authors have no evidence for the source of the missing signals. Second, even if they are wing margin Wnts, there is no evidence that this can control MT polarity. Instead, the quoted work suggests a fairly direct interaction between Wnts and core protein activity, and there is no evidence that changing core protein activity can orient MTs. I think the comments should take this into account. Or the authors could test this by overexpressing Wnt4 and looking.

Reviewer 3: It seems unlikely that Wnt is functioning with Core proteins in a 'non-canonical' pathway as well as acting upstream to control MT orientation.

Wu et al showed that Wnt 4 and Wg (or at least Wnt4 plus some other Wg dependent signal) influence polarity in the distal part of the wing. However, the data on which they base their model that this occurs by affecting Fz-Vang interaction should be taken with a grain of salt, as the assay depended on a cell culture model with high concentrations of added Wnt, and the physiological relevance is therefore unclear. Furthermore, their model would require that concentrations of ligand are sufficiently different across a single cell diameter to influence polarity outcomes, also a problem of questionable plausibility. Therefore, we feel it is valuable to consider other possibilities. And, of course, yet other signals may be at play.

With respect to Wnt4, we do indeed see an ability to modify MT orientation, and would therefore like to at least suggest the possibility of a different mechanism. This alternative would not necessarily be mutually exclusive, though it might stretch plausibility to suggest that Wnts work by two distinct mechanisms.

We have included the data for this, and elaborated some in the discussion, while attempting to minimize unnecessarily controversial assertions.

https://doi.org/10.7554/eLife.02893.026

Article and author information

Author details

  1. Maja Matis

    Department of Pathology, Stanford University School of Medicine, Stanford, United States
    Present address
    Institute of Neurobiology and Behavioral Biology, University of Münster, Münster, Germany
    Contribution
    MM, Conception and design, Acquisition of data, Analysis and interpretation of data, Drafting or revising the article
    For correspondence
    matism@uni-muenster.de
    Competing interests
    The authors declare that no competing interests exist.
  2. David A Russler-Germain

    Department of Pathology, Stanford University School of Medicine, Stanford, United States
    Present address
    Washington University School of Medicine, St. Louis, United States
    Contribution
    DAR-G, Acquisition of data, Analysis and interpretation of data
    Competing interests
    The authors declare that no competing interests exist.
  3. Qie Hu

    Department of Electrical Engineering and Computer Sciences, University of California, Berkeley, Berkeley, United States
    Contribution
    QH, Wrote the simulation model and performed simulations
    Competing interests
    The authors declare that no competing interests exist.
  4. Claire J Tomlin

    Department of Electrical Engineering and Computer Sciences, University of California, Berkeley, Berkeley, United States
    Contribution
    CJT, Wrote the simulation model and performed simulations
    Competing interests
    The authors declare that no competing interests exist.
  5. Jeffrey D Axelrod

    Department of Pathology, Stanford University School of Medicine, Stanford, United States
    Contribution
    JDA, Conception and design, Drafting or revising the article
    Competing interests
    The authors declare that no competing interests exist.

Funding

National Institutes of Health (GM059823)

  • Jeffrey D Axelrod

National Institutes of Health (GM097081)

  • Jeffrey D Axelrod

National Institutes of Health (GM107615)

  • Jeffrey D Axelrod

Deutsche Forschungsgemeinschaft (EXC1003)

  • Maja Matis

AXA Research Fund

  • Maja Matis

The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.

Acknowledgements

We thank Seth Blair, David Strutt, Kenneth Irvine, Vladimir Gelfand and the Developmental Studies Hybridoma Bank for reagents; Mike Simon and Axelrod lab members for critical readings of the manuscript. MM was generously supported by a postdoctoral fellowship from the AXA Research Fund. Supported by NIH grants GM059823, GM097081 and P50 GM107615 (J Ferrell PI) to JDA.

Reviewing Editor

  1. Helen McNeill, Reviewing Editor, The Samuel Lunenfeld Research Institute, Canada

Publication history

  1. Received: March 25, 2014
  2. Accepted: August 9, 2014
  3. Accepted Manuscript published: August 14, 2014 (version 1)
  4. Version of Record published: September 2, 2014 (version 2)

Copyright

© 2014, Matis et al.

This article is distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use and redistribution provided that the original author and source are credited.

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