In a wildtype neuromast, each afferent neuron only innervates HCs with apical hair bundles polarized in one of the two orientations (Nagiel et al., 2008; Faucherre et al., 2009; Pujol-Martí et al., 2014). Emx2 is also expressed in HCs of just one orientation (Jiang et al., 2017). Based on these results, we hypothesized that each afferent neuron should only innervate either Emx2 positive or negative HCs within a neuromast (Figure 1A–B). To test this hypothesis, we injected a neuroD:tdTomato plasmid into transgenic myo6b:actb1-GFP zebrafish embryos. This enabled us to visualize single afferent neurons labeled with tdTomato innervating a neuromast and the orientation of hair bundles labeled with Actb1-GFP. Figure 1 illustrates two such examples of wildtype neuromasts in the primary posterior lateral line (Figure 1C–J,K–R). These neuromasts contain HCs oriented along the anterior-posterior axis of the body. As previously demonstrated, in these neuromasts, Emx2 immunoreactivities are only detected in mature HCs with hair bundles oriented towards the posterior direction (A > P, Figure 1C,F–J,K,N–R; Jiang et al., 2017). Emx2 is also expressed in immature HCs that can be identified by weak GFP signals and/or incomplete bundle polarity establishment. Only one of the immature HCs within a pair expresses Emx2 (Figure 1C–R, yellow arrow). Notably, we found that each single-labeled neuron either associated with all the Emx2-positive HCs in a neuromast (example, Figure 1C–J), or associated with all the Emx2-negative HCs in a neuromast (example, Figure 1K–R). Based on the association of single afferent neurons with HCs that were either Emx2-positive or-negative, we hypothesized that Emx2, which is required for establishing the hair bundle orientation (Jiang et al., 2017), may also be involved in regulating the pattern of neuronal innervation.

To test the above hypothesis, we investigated the neuronal innervation pattern in neuromasts of loss and gain of emx2 function zebrafish. We first generated wildtype and emx2 mutant fish in an HGn39D transgenic background, in which all afferent neurons innervating each neuromast are GFP-positive (Nagayoshi et al., 2008; Faucherre et al., 2009). We then injected these embryos with neuroD:tdTomato to label individual afferent neurons. This enabled us to examine the innervation pattern of single neurons in the context of the entire afferent processes beneath each neuromast. In wildtype neuromasts, fibers of a single-labeled neuroD:tdTomato-positive neuron only overlapped with a subset of the HGn39D-GFP-positive afferents and ramified approximately one half of the neuromast (Figure 2A–D). By contrast, emx2 ko neuromasts, in which all HCs are oriented towards the anterior direction (Figure 2E,I, P > A), showed an altered neuronal branching pattern (Figure 2F–H,J–L). The majority of the single neurons in emx2 ko neuromasts showed a broader distribution (Figure 2G), when compared to controls (Figure 2B–D). Despite these broader distributions, there were always some GFP-positive nerve endings that did not overlap with tdTomato signals (Figure 2F–H, circles). Additionally, a smaller proportion of single fibers overlapped with less than half of the GFP-positive nerve endings in emx2 ko neuromasts (Figure 2J–L), when compared to controls (Figure 2B–D). We quantified the average percentage of overlap between tdTomato- and GFP-positive areas and found that in wildtype fish, the overlap by a single neuron is consistently around 50% (Figure 2U, Figure 2—source data 1). In contrast, single neurons in emx2 ko clearly segregated into two populations and showed either dramatically more (70%) or less (20%) overlap than the wildtype neurons (Figure 2U, p=0.0016 for emx2 ko major, p=0.0012 for emx2 ko minor). Based on these measurements, we named the two populations major and minor axons, respectively (Figure 2U). Similar major (Figure 2N–P,U, p=0.0006) and minor (Figure 2R–T,U, p=0.0005) branching patterns were observed for emx2 gof neuromasts, in which all HCs are oriented in the A > P direction (Figure 2M,Q). The altered branching pattern of a single afferent neuron in both emx2 ko and gof mutants suggests that in addition to establishing hair bundle orientation, Emx2 also regulates the pattern of neuronal innervation.

Figure 2

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Percentages of tdTomato-positive area per total GFP-positive area.

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To investigate whether the changes in the branching pattern of individual neurons in emx2 mutants represent a change in the number of HCs innervated, we conducted similar single-neuron labeling experiments using the myo6b:actb1-GFP transgenic line to more definitively correlate the relationship between nerve endings and HC bodies. We defined nerve endings that juxtaposed the basal region of HCs as contacts between the HC and the afferent. Figure 3A–D3 illustrates a wildtype neuromast, in which a single afferent contacts all the HCs that are in a P > A orientation (Figure 3A–C, 4 out of 9 total HCs, Figure 3D-D3, arrowheads, Table 1, 52.9%, Table 1—source data 1). Similar contacts between nerve endings and HCs were found in emx2 mutants (Figure 3E-T2). In emx2 ko, major afferent neurons contacted more than half (Figure 3E–H3, 8 out of 10 total HCs, Table 1, 74.8%, p=5.19E-20, Table 1—source data 1) while minor afferent neurons contacted less than half of the total number of HCs within a neuromast (Figure 3I–L3, 4 out of 13 HCs, Table 1, 25.4%, p=1.41E-21, Table 1—source data 1). Similar to emx2 ko afferents, major and minor neurons contacted a significantly more and fewer HCs respectively in emx2 gof neuromasts compared to wildtype afferents (Example major, Figure 3M-P3, 10 out of 12 HCs, arrowheads, Table 1, 75.2%, p=1.82E-25; example minor, Figure 3Q-T2, 3 out of 11 HCs, arrowheads, Table 1, 25.8%, p=1.08E-18, Table 1—source data 1). However, in emx2 mutants, the nerve endings of both major and minor neurons were juxtaposed to HC bodies (Figure 3H1–H3, L1–L3, P1–P3, T1–T2, arrowheads) similar to controls (Figure 3D1–D3), suggesting that they were successfully making HC contacts. We also examined the frequency of major and minor single afferent neurons obtained using single fiber labeling and found they were in an approximate respective ratio of 3:2, for both emx2 ko and gof neuromasts (Table 1). Overall these results indicate that in emx2 mutants both major and minor neuronal fibers make contacts with HCs that are similar to those found in wildtype. Based on these similarities, it is likely that these contacts in emx2 mutants may represent synapses.

Figure 3

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To determine whether all afferent nerve endings form synapses with HCs in emx2 mutants, we analyzed emx2 mutants using an antibody to a pre-synaptic protein, RibeyeB. In wildtype larvae, afferent fibers are associated with presynaptic RibeyeB staining (Figure 4B–D3). A single afferent neuron appears to innervate all the A > P or P > A HCs in the neuromast, and afferents are associated with RibeyeB-labeled presynapses (Example A > P, Figure 4A,C–D). In both emx2 ko and gof neuromasts, we observed that major as well as minor afferent neurons associated with RibeyeB-labeled presynapses (Figure 4E–T3, white arrows). However, we also observed both major and minor afferent nerve endings that were adjacent to presynapses but failed to directly associate (Figure 4E–T3, white arrowheads). When we quantified the number of RibeyeB puncta that were colocalized with tdTomato-positive nerve endings per HC, we found that this number was not changed for the major fibers, but significantly decreased for the minor fibers for both loss- and gain-of-emx2 function neuromasts (Figure 4—source data 1, p=0.069 for emx2 ko major, p=0.007 for emx2 ko minor, p=0.383 for emx2 gof major, p=0.002 for emx2 gof minor). We also quantified the degree of colocalization or the proportion of presynaptic RibeyeB label that overlapped with the afferent-fiber label using Mander’s colocalization analysis. Consistent with fewer RibeyeB puncta associating with afferent fibers, the Mander’s colocalization coefficients were also decreased in minor fibers of emx2 mutants compared to wildtype (Figure 4—source data 2, p=0.159 for emx2 ko major, p=0.048 for emx2 ko minor, p=0.011 for emx2 gof major, p=0.037 for emx2 gof minor). Together, these results suggest that a majority of the afferent nerve endings in emx2 mutants and wildtype are associated with presynapses. However, the presence of nerve endings juxtaposed to HC bodies that do not associate with presynapses (incomplete synapses) are more prevalent in the emx2 mutants than in wildtype (Sheets et al., 2017), primarily in the minor fibers.

Figure 4

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Quantification of colocalization between RibeyeB and tdTomato-positive nerve endings per HC.

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Figure 4—source data 2

Mander's coefficient of RibeyeB and tdTomato colocalization.

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To further assess synapse formation, we examined RibeyeB immunoreactivities in conjunction with the postsynaptic protein, Maguk (membrane associated guanylate kinases), in wildtype and emx2 mutants. Previous work has demonstrated that this co-label can reliably be used to quantify complete and incomplete synapses in neuromasts (Sheets et al., 2011; Sheets et al., 2017). In wildtype neuromasts (Figure 5A–D2), the majority of RibeyeB and Maguk puncta were juxtaposed with each other, and based on this co-label, we observed on average three complete synapses per HC (Figure 5M; Sheets et al., 2017). Similar numbers of complete synapses per HC in both emx2 ko and gof mutants were observed (Figure 5E–H2, I–L2, M, p=0.103 for emx2 ko, p=0.878 for emx2 gof, Figure 5—source data 1). We also used Mander’s colocalization analysis to quantify the proportion of RibeyeB label that overlapped with Maguk label. Using this analysis, we found no difference in emx2 mutants, compared to wildtype (Figure 5—source data 2).

Figure 5

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Figure 5—source data 1

Quantification of colocalized RibeyeB and Maguk puncta per HC.

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Figure 5—source data 2

Mander's coefficient of RibeyeB and Maguk colocalization.

https://doi.org/10.7554/eLife.35796.013

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Figure 5—source data 3

Quantification of total number of RibeyeB and Maguk puncta per HC.

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Figure 5—source data 4

Percentages of solitary RibeyeB and Maguk puncta per neuromast.

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Although there is no difference in complete synapse number and overall pre-and post-synaptic colocalization, emx2 mutant neuromasts showed an increase number of both total RibeyeB and Maguk per HC (p=6.09E-05 for RibeyeB of emx2 ko, p=2.09E-04 for RibeyeB of emx2 gof, p=3.35E-04 for Maguk of emx2 ko, p=0.567 for Maguk of emx2 gof, Figure 5—source data 3). This was due to an increase in individual RibeyeB and Maguk puncta that were not juxtaposed with each other (Figure 5H1–H2, L1–L2, white and yellow arrows). We quantified the percentage of solitary RibeyeB or Maguk puncta per neuromast and found that there were significantly more solitary puncta in both emx2 ko and gof mutants compared to controls (Figure 5H–H2,L–L2, N, p=5.05E-07 for RibeyeB of emx2 ko, p=1.35E-08 for RibeyeB of emx2 gof, p=9.98E-09 for Maguk of emx2 ko, p=0.033 for Maguk of emx2 gof, Figure 5—source data 4). The uncoupling of pre- and post-synaptic components support that idea that in addition to forming authentic synapses, emx2 mutants also have failures in synapse formation. Therefore, we asked whether afferent neurons in emx2 mutants are functionally active, by measuring neuronal responses during hair bundle displacements in emx2 mutants.

To determine whether emx2 mutant afferent neurons are functional, we used in vivo calcium imaging and electrophysiology to measure afferent neuron activity. We used a waterjet to directionally stimulate HCs within a neuromast in either an anterior or posterior direction while simultaneously imaging postsynaptic calcium signals or recording spikes.

We used GCaMP6s to image calcium signals in the afferent process directly beneath the neuromast HCs during a 500 ms waterjet stimulation (Figure 6). In wildtype, we observed robust calcium signals in the innervating afferent process during both A > P and P > A directed waterjet stimulation (Figure 6A,A’). In wildtype afferents, calcium responses to each directional stimulation (A > P or P > A) occurred in distinct domains of the afferent process (Figure 6A,A’). In contrast, calcium signals were only observed in response to P > A stimulation in emx2 ko afferents (Figure 6B’). Inversely, calcium signals were only detected in response to A > P stimulations in emx2 gof afferents (Figure 6C). No afferent calcium signals were observed in emx2 ko mutants during A > P stimuli (Figure 6B) or in emx2 gof mutants during P > A stimuli (Figure 6C’). These results indicate that HCs and afferent neurons in emx2 mutants are functional and directionally selective. Our results are also consistent with the single-directional sensitivity of the emx2 gof (A > P) hair bundles compared to wildtype hair bundles in both A > P and P > A directions (Jiang et al., 2017). We quantified the magnitude of the calcium signal in the entire afferent process for each stimulus. We found that for the A > P stimulus, the emx2 gof calcium signals were 41% higher compared to wildtype (Figure 6D,D’, p=0.027, Figure 6—source data 1). Similarly, in emx2 ko fish, the P > A calcium signals were 58% higher compared to wildtype (Figure 6E,E’, p=0.0003, Figure 6—source data 1). These results suggest that compared to wildtype, in emx2 mutants, afferents are able to recruit additional HCs to respond to their respective direction of stimulus.

Figure 6

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Figure 6—source data 1

Magnitude of afferent calcium signals per Neuromast.

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Figure 6—source data 2

Magnitude of afferent calcium signals per HC.

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To investigate whether there are differences in the synaptic transfer between individual HCs of wildtype and mutants, we quantified the magnitude of the afferent calcium signals per HC. To identify HCs within the neuromast, we used FM 4–64 to label the HCs after afferent calcium imaging (Figure 6A’’,B’’,C’’). Then we measured the magnitude of calcium signals contained within 3 µm regions of interest (ROIs) on the afferent process beneath each functional HC (Figure 6A’’,B’’,C’’). Using this approach, we found that per HC, the magnitude of the afferent calcium signal was the same compared to wildtype (Figure 6F,G, A > P direction: GCaMP6 ∆F/F, wildtype 70.5%, emx2 ko 71.6%, p=0.99; P > A direction: GCaMP6 ∆F/F, wildtype 51.6%, emx2 gof 73.4%, p=0.48, Figure 6—source data 2). This suggests that the overall properties of each HC-afferent contact are not dramatically altered in emx2 mutants.

Although calcium imaging provides an excellent overview of the response properties within the entire afferent process beneath an individual neuromast, our imaging approach does not have the sensitivity to detect and resolve the timing of single action potentials. Therefore, it is possible that there were evoked responses in the off -stimulus direction (ie: A > P direction in emx2 ko) that we could not detect using calcium imaging. To address this possibility, we performed in vivo electrophysiological recordings from the afferent cell bodies in the posterior lateral line ganglion, while stimulating neuromast HCs with a waterjet.

In wildtype larvae, within each neuromast, each afferent neuron contacts multiple HCs with either an A > P or P > A directional sensitivity (Figure 1B; Nagiel et al., 2008; Faucherre et al., 2009). Consistent with this sensitivity pattern, during a 500 ms waterjet stimulus, we were able to record trains of action potentials (spikes) either during A > P or P > A stimuli in wildtype afferents (Figure 7A,B, wildtype, A > P, 5/15, 33%, P > A, 10/15, 66%, n = 15 afferent neurons, Figure 7—source data 1). When these same wildtype afferents were stimulated in the opposite directions (off-stimulus direction), the average spike number was dramatically reduced (Figure 7B’). When we recorded spikes in emx2 mutant afferent neurons, we only identified P > A afferents in emx2 ko mutants (n = 8/8 neurons; Figure 7B) and A > P afferents in emx2 gof mutants (n = 7/7 neurons; Figure 7B). The number of spikes in the on-stimulus direction, in emx2 mutants was not greater than wildtype (wildtype versus emx2 ko, p=0.65; wildtype versus emx2 gof, p=0.74). When emx2 mutant afferents were stimulated in the off-stimulus direction, similar to wildtype afferents, the spike numbers were dramatically reduced (Figure 7B’). Together, our calcium imaging and electrophysiological results both indicate that the afferent neurons in emx2 mutants are functional and respond in a predicted manner according to their hair bundle orientation.

Figure 7

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Figure 7—source data 1

Average spikes per 10, 500 ms step stimuli.

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Thus far, our results support the idea that Emx2 expressed in HCs is required for establishing directional selectivity of afferent neurons, in addition to determining hair bundle orientation (Jiang et al., 2017). Next, we asked whether it was hair bundle orientation per se or the identity of the HC conferred by Emx2 that is important to establish afferent selectivity. To address this question, we investigated a core planar cell polarity mutant, vangl2^m209, in which a recessive frameshift mutation in vangl2 results in a functional null protein (Solnica-Krezel et al., 1996; Jessen et al., 2002). Hair bundles in neuromasts of vangl2^m209 are misoriented due to misalignment of the basal body and in turn the associated kinocilium, which directs bundle orientation during development (Figure 8E,M,P; López-Schier and Hudspeth, 2006). Although emx2 mutants have misoriented hair bundles in both the inner ear and neuromasts, the orientations are not random as in the Vangl mutants. Importantly in both mutants, the misoriented hair bundles are attributed to mis-localization of the kinocilium (Jiang et al., 2017). Based on the implication of the mis-located basal body/kinocilium in both of these mutants, we asked whether the neuronal innervation is affected in vangl2^m209. First, we investigated whether Emx2 is expressed in vangl2^m209. Our results showed that although hair bundle orientation is random in vangl2^m209 mutants, Emx2 is still expressed in half of the HCs within a neuromast (Figure 8E–H2, example 4/8 HCs, Figure 8I, p=0.67, Figure 8—source data 1), similar to controls (Figure 8A–D2, example 6/12 HCs, Figure 8I). The maintenance of 50% of Emx2-positive HCs in vangl2^m209 mutants suggests that hair bundle misorientation in this mutant is independent of emx2 (Figure 8I). Furthermore, the hair bundle orientation of double mutants of vangl2^m209 with emx2 ko or gof was also random (Figure 8N,O). The orientation defects in the double mutants resembled defects in vangl2^m209 (Figure 8M), rather than the unidirectional orientation phenotype observed in emx2 ko and gof single mutants (Figure 8K,L). Therefore, these genetic analyses indicate that vangl2 is epistatic to emx2.

Figure 8

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Ratio of Emx2-positive HCs within a neuromast.

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Figure 8—source data 2

Ratio of innervated HCs to total number of HCs.

https://doi.org/10.7554/eLife.35796.023

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The above results demonstrate that the vangl2 mutant is a good model to address the question whether hair bundle orientation per se is coupled to neuronal selectivity since hair bundle misorientation in this mutant is independent of emx2. When we examined the innervation patterns of single afferent neurons in vangl2^m209 neuromasts, we observed that Emx2-mediated afferent selectivity was preserved. For example, a single afferent neuron can selectively innervate Emx2-positive HCs (Example, Figure 8P–U, 5 out of 12 total HCs, circles). In addition, the ratio of the number of HCs innervated by a single neuron within a neuromast is similar to wildtype (Figure 8Y, p=0.26, Figure 8—source data 2). Importantly, single neurons were able to select and contact only the Emx2-positive HCs (Figure 8T–X), despite the misoriented hair bundles. These results indicate that neuronal innervation in neuromasts occurs independent of hair bundle orientation and is directed by Emx2.

In a wildtype neuromast, a single afferent neuron innervates only HCs with bundles that are oriented in the same direction, which constitute about half of the total number of HCs. In emx2 ko and gof neuromasts, in which all HCs have uni-directionally oriented bundles, we found that one population of afferent neurons can innervate more than half of the total number of HCs. These results suggest that these neurons have the capacity to innervate additional HCs of similar orientation based upon their availability. Nevertheless, our results also suggest that there is an upper limit to this capacity since a single neuron was unable to innervate all the HCs within a ko or gof emx2 mutant neuromast. Coincidently, we also observed a smaller portion of single neurons innervating less than half of the total number of HCs in the emx2 mutant neuromasts (Table 1).

What determines whether a neuron forms a major versus a minor innervation pattern in the mutant neuromasts? At least two models are consistent with our observations. We refer to these models as ‘exclusive’ and ‘inclusive’ based on the role of Emx2 in determining neuronal selectivity. In the exclusive model, the transcriptional activity downstream of Emx2 in HCs is sufficient to direct afferent innervation and determine the directional selectivity of each neuron (Figure 9). In this model, there are no other cues within neuromasts or among the lateral line ganglion neurons that influence this decision, at least not initially. However, interaxonal cross-inhibition could occur after the initial contact with HCs that refines or maintains the segregated pattern (Changeux and Danchin, 1976; Deppmann et al., 2008; Mizumoto and Shen, 2013). In this scenario, major and minor afferents in emx2 mutants could arise due to timing; axons arriving at the neuromast first may innervate many cells and become major afferents. In contrast, axon that arrive slightly later may find fewer available HCs to innervate and thus become minor afferents.

Figure 9

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In the inclusive model, Emx2, though important, is not the only factor regulating neuronal selectivity (Figure 9). For example, both pre- and post-synaptic signaling may be important to determine neuronal selectivity. In this scenario, major and minor innervation patterns in the emx2 mutants may arise from the fact that afferent neurons that innervate A > P HCs (A > P neurons) are molecularly distinct from those that innervate P > A HCs (P > A neurons). In support of this notion, neurons that innervate Emx2-positive and -negative HCs in the mammalian maculae of the inner ear are most likely different from each other because their central axons project to different regions of the brain (Maklad et al., 2010). Therefore, neurons that innervate Emx2-positive and negative HCs in the lateral line system may also be molecularly different, similar to the neurons of the mouse maculae. Additionally, ample evidence from other systems indicates that specific synapse formation often requires partnering between pre- and post-synaptic signaling molecules such as ephrin-eph, semaphorin-plexin and other adhesion molecules (for review see, Sanes and Yamagata, 2009; Margeta and Shen, 2010; Williams et al., 2010; Yogev and Shen, 2014). The selective innervation pattern of the lateral line afferent neurons may be analogous to other pre- and postsynaptic neuronal pairing, requiring a match between the HCs (expressing downstream effectors of Emx2 or the lack thereof) and respective molecular determinants from the postsynaptic afferent neurons. Moreover, the described interactions of cellular processes between nascent HCs and afferent nerve terminals of a neuromast during synaptogenesis also provide some morphological evidence that there could be specific HC-neuron coupling (Dow et al., 2015).

Under the above inclusive scenario, the P > A neurons in the emx2 ko neuromasts identify molecular cues from an expanded number of P > A HCs and become major afferents, whereas the A > P neurons are unable to identify their molecular cues, since A > P HCs are absent (Figure 9). Without a molecular target, these A > P neurons either form only a few synapses with P > A HCs or fail to form any synapses at all and become minor afferents. Likewise, in the emx2 gof neuromasts, the A > P neurons expand their innervation pattern to accommodate the increase in A > P HCs and become major afferents, while the P > A neurons in the emx2 mutant form minor innervation patterns. Previous axotomy studies showed that when all axons innervating a single neuromast were severed except one, the single remaining neuron was able to expand its innervation to HCs of the opposite orientation (Pujol-Martí et al., 2014). As a result of this expanded innervation, the remaining neuron responded to hair bundle deflections from two directions instead of one. If we assume that there are indeed two types of neurons innervating a given neuromast, then the axotomy data taken together with our data on emx2 mutants suggest that other permissive factor(s) in addition to Emx2 instruct synapse formation and can expand innervations beyond their intended targets. Nevertheless, the inclusive model is not limited to molecular differences between neurons and could include other determinants from HCs and/or supporting cells. Furthermore, under either the inclusive or exclusive model, we postulate that the main source of Emx2 for neuronal selectivity resides in the HCs because we cannot detect measurable emx2 mRNA or protein in the lateral line ganglion using in situ hybridization or immunostaining.

Despite the altered innervation pattern observed in the emx2 mutant neuromasts, our calcium imaging and extracellular neuronal recording results indicate that these neurons respond in the predicted manner according to the orientation of the HCs that they innervate; neurons of the emx2 ko neuromasts only respond to stimulation in the P > A direction because only P > A HCs are present. Likewise, neurons of emx2 gof neuromasts only respond to hair bundle stimulation in the A > P direction.

Despite the increase in the amplitude of post-synaptic calcium signals within the entire afferent terminal in emx2 mutant compared to controls, this increase did not translate into more evoked spikes at the level of a single afferent neuron, even though some of the neurons innervated more HCs than normal. What could account for these seemingly paradoxical results? It is possible that the increase in calcium signaling is not sufficient to elicit a change in spike number at the cell body level. It is also possible that due to the variability in our electrophysiology data, it may not be possible to resolve an overall increase in spike number in emx2 mutant neurons. For example, the average number of spikes recorded from a single wildtype neuron shows a large range from 1 to 21 spikes (averages for 10 repeated 500 ms stimuli). It is not clear whether these differences represent a heterogenous population of neurons with different receptive fields. For example, if a single neuron innervates multiple neuromasts (large receptive field) it may only show a few spikes when only one of its neuromasts is stimulated, whereas a neuron that innervates only one neuromast (small receptive field) may respond with a large number of spikes when that neuromast is stimulated. Without the ability to further delineate the diverse types of neurons in wildtype and compare them directly to their counterparts in emx2 mutants, it is not possible to determine whether the increase in post-synaptic calcium affected evoked spike numbers in the neuronal cell body. Furthermore, while our anatomical and physiological results indicate that afferent neurons in the emx2 mutants are responding in a predicted manner, our results cannot distinguish functional differences between major versus minor afferents.

The observed changes in neuronal innervation patterns in the emx2 mutants are consistent with the changes in hair bundle orientation, suggesting that the transcriptional activity of Emx2 mediates both hair bundle orientation and selectivity of neuronal innervation. However, results from the vangl2^m209 mutants suggest that neuronal selectivity is not dependent on hair bundle orientation per se. Although the mechanism of hair bundle misorientation in both vangl2^m209 and emx2 mutant mice may share a common pathway (López-Schier and Hudspeth, 2006; Jiang et al., 2017), the neuronal innervation pattern in vangl2^m209 remains consistent with the Emx2 expression pattern of HCs. These results suggest that Emx2 regulates both hair bundle orientation and neuronal innervation patterns, whereas Vangl2 only regulates hair bundle orientation, suggesting that these two cellular processes are independently regulated.

Our results indicate that Emx2 expression in HCs of neuromasts is not affected in the vangl2^m209 (Figure 8) and similarly, Vangl2 expression is not affected in Emx2 ko mouse inner ears (Jiang et al., 2017), further supporting that these proteins are independently regulated. However, our genetic analyses indicate that vangl2 function is epistatic to emx2 with regards to hair bundle orientation. These results are consistent with results in the mouse utricle indicating that a core planar cell polarity protein such as Vangl2, functions in an intercellular manner and regulates an intracellular signaling mechanism such as Emx2 (Montcouquiol et al., 2006; Yin et al., 2012; Copley et al., 2013; Jiang et al., 2017).

Taken together our results indicate that the restricted expression of Emx2 to half of the HCs within a neuromast reverses the hair bundle orientation by 180 degrees and allows the detection of water flow from the opposite direction (Jiang et al., 2017). In addition, the expression of Emx2 guides neuronal patterning and preserves the directional selectivity of the HCs. Thus, Emx2 regulates the two key components that confer directional selectivity in the peripheral lateral line system. Given the conserved role of Emx2 in mediating hair bundle orientation among mechanosensory organs of fish and mammals (Jiang et al., 2017), its role in regulating post-synaptic partner described here may apply to other neural systems where Emx2 is normally expressed such as the cortex and olfactory epithelium (Cecchi and Boncinelli, 2000; Cecchi, 2002; Nédélec et al., 2004).

Adult zebrafish (Danio rerio) were maintained with a 14 hr light, 10 hr dark cycle. Zebrafish protocols were approved by the Animal User Committee at the National Institutes of Health (Animal study protocol #1362–13). Zebrafish larvae were raised in E3 embryo media as follows: 5 NaCl, 0.17 KCl, 0.33 CaCl2, and 0.33 MgSO4, buffered in HEPES, at 28.5°C. Previously described transgenic zebrafish strains used in this study include the following: Tg(myo6b:actb1-GFP)^vo8Tg (RRID:ZFIN_ZDB-GENO-120926-20), Tg(cntnap2a)^nkhgn39dEt or HGn39D (RRID:ZFIN_ZDB-GENO-100113-50), Tg(myo6b:emx2-p2a-nls-mCherry)^idc4Tg (RRID:ZFIN_ZDB-GENO-170619-3), emx2^idc5 (emx2 ko) (RRID:ZFIN_ZDB-ALT-170606-5), vangl^m209 (RRID:ZFIN_ZDB-GENO-100615-1), Tg(hsp70l:GCaMP6s-CAAX-SiLL1)^idc8Tg (Solnica-Krezel et al., 1996; Jessen et al., 2002; Nagayoshi et al., 2008; Kindt et al., 2012; Jiang et al., 2017; Zhang et al., 2018). F1 to F3 generation of emx2 gof (myo6b:emx2-p2a-nls-mCherry) were used in our study, and incomplete penetrance of the hair bundle phenotype in neuromasts from F2 and F3 generations have been observed. Larvae were used between 3–6 dpf.

To label a single afferent neuron, neuroD:tdTomato plasmid was used, in which a 5 kb minimal promoter of neurod drives tdTomato expression (Toro et al., 2015). NeuroD:tdTomato plasmid at a concentration of 50 ng/ul was pressure injected to one-cell stage zebrafish embryos. Larvae were screened at 2–3 dpf (days post fertilization) for tdTomato expression in the posterior lateral line axon using a SteREO Discovery V20 microscope with an X- Cite 120 external fluorescent light source (EXFO Photonic Solutions Inc., Ontario, Canada). After selection of candidates, definitive expression in the posterior lateral line axon was ascertained using a 63X oil immersion objective on a Zeiss LSM780 confocal microscope (Carl Zeiss Ltd. Cambridge, UK).

Zebrafish larvae as 3–4 dpf were anesthetized with 0.03% ethyl 3-aminobenzoate methanesulfonate (Sigma, #MS-222, St Louis, MO) and embedded in 1.5% low melting point agarose containing 0.01% tricaine, and then imaged at 63X using a Zeiss LSM780 confocal microscope.

For staining zebrafish larvae, 3–6 dpf embryos were fixed with 4% paraformaldehyde in PBS for 3.5 hr at 4°C. Post-fixed larvae were rinsed with 0.05% Tween-20 PBS (PBT) and treated with pre-chilled acetone at - 20°C. Then, larvae were incubated with a blocking solution (2% goat serum, 1% BSA in PBT) for 2 hr at room temperature or overnight at 4°C, followed by incubation with primary antibodies diluted in blocking solution for 2 hr at room temperature or overnight at 4°C. Larvae were washed four times with PBT for 5 min each before incubating with secondary antibodies at 1:1000 dilution in blocking solution for 2 hr at room temperature. Then, larvae were washed and mounted with Anti-fade and imaged with a Zeiss LSM780 confocal microscope. For whole-mount immunofluorescence labeling, we used the following primary antibodies: rabbit anti-Emx2 (1:250; KO609, Trans Genic, Fukuoka, Japan), mouse anti-RibeyeB (1:1000) (Sheets et al., 2011), and mouse anti-Maguk clone K28/86 (1:500; NeuroMab, Davis, CA, RRID:AB_2292909). To detect F-actin, we stained with fluorescein or Alexa Fluor 647 phalloidin (1:50; Thermo Fisher Scientific, Carlsbad, CA, RRID:AB_2620155).

To suppress muscle activity and movement for functional analyses, larvae were anesthetized with 0.03% ethyl 3-aminobenzoate methanesulfonate (MS-222) in E3, and mounted onto Sylgard (Dow Corning) filled dishes using tungsten pins. After larvae were anesthetized, they were then microinjected in the heart with 125 μM α-bungarotoxin (Tocris) to suppress muscle activity. After microinjection, larvae were then rinsed thoroughly to remove MS-222, and maintained in extracellular solution in mM: 130 NaCl, 2 KCl, 2 CaCl₂, 1 MgCl₂ and 10 HEPES, pH 7.3, 290 mOsm. To stimulate lateral-line HCs we used a pressure clamp (HSPC-1, ALA Scientific, New York) attached to a glass or waterjet micropipette (inner tip diameter ~30–50 μm) filled with extracellular solution. The waterjet was positioned (MP-265, Sutter Instruments) approximately 100 μm from a given neuromast. The waterjet was placed in focus in the plane of the kinocilial tips. Displacement (~5 μm) of the kinocilial tips was verified by measuring the distance moved during the displacement. To trigger the waterjet during recordings of lateral-line afferents (see below), the pressure clamp was driven by a voltage command delivered by the recording amplifier. For afferent calcium imaging experiments, the pressure clamp was driven by a voltage step command. This voltage command was generated in the Prairie View (Bruker Corporation) imaging software during calcium imaging.

The method for recording postsynaptic action currents has been described previously (Olt et al., 2016; Sheets et al., 2017). All recordings were performed in extracellular solution (see above), on afferent neurons innervating zebrafish primary neuromasts (L1–L4). For the extracellular recordings, borosilicate glass pipettes were pulled (P-97, Sutter Instruments) with a long taper to obtain resistances between 5 and 10 MΩ in extracellular solution. Signals were collected with a Multiclamp 700B, a Digidata 1550 data acquisition board, with pClamp10 software (Molecular Devices, LLC). Extracellular currents were acquired from lateral-line afferent neuron in the loose-patch configuration (seal resistances ranged from 20 to 80 MΩ in extracellular solution). Recordings were done in voltage-clamp mode, sampled at 50 μs/pt, and filtered at 1 kHz. To identify the neuromast innervating an afferent neuron, the fluid-jet was used to progressively stimulate primary neuromasts of the posterior lateral line until phase-locked spiking was detected.

Calcium imaging experiments were performed in extracellular solution (see above). Afferent calcium measurements were made at postsynaptic sites directly beneath HCs using hsp70l:GCaMP6s-CAAX-SiLL1 transgenic fish. Acquisitions were made on an upright Swept-field confocal system (Bruker Corporation) with a 60X 1.0 NA CFI water-immersion objective (Nikon, Tokyo, Japan). The Swept-field microscope used a Rolera EM-C2 EMCCD camera (QImaging) controlled using Prairie view (Bruker Corporation). GCaMP6s-CAAX was excited using a 488 nm solid-state laser. To image calcium activity within the entire post-synaptic process simultaneously across the Z-axis, we used piezoelectric motor (PICMA P-882.11–888.11 series, PI instruments) attached to the objective. The piezo allowed rapid imaging in five planes along the Z-axis every 2 μm at a 50 Hz frame rate, enabling a 10 Hz volume rate. Our five plane Z-stacks were later projected into one plane for further image processing and quantification (see below). After functional calcium imaging, each larva was incubated in 3 µM FM 4–64 (Thermo Fisher Scientific) in E3 for 30 s, followed by 3 E3 washes, to label HCs. Confocal images of afferent process and FM 4–64 labeled HCs were then acquired on an upright Nikon C2 laser-scanning confocal microscope using a 60X 1.0 NA water objective lens. Appropriate solid-state lasers were used to image and excite GCaMP6s and FM 4–64.

Afferent electrophysiology recordings were analyzed with software written in Igor Pro (Wavemetrics) and were plotted with Igor Pro and Prism 7 (Graphpad). For afferent GCaMP6s-CAAX calcium measurements, the raw images were processed using a custom program in Matlab (MathWorks, Source code 1–3). For this analysis, we removed the first 10 images to reduce the effect of photobleaching. Then the raw images were registered to reduce movement artifacts by applying efficient subpixel image registration based on cross-correlation (Zhang et al., 2016). Then the spatial calcium signals were converted to heat maps as previously described (Zhang et al., 2016). Briefly, we first computed the baseline image (or reference image or F₀) by averaging the images during the pre-stimulus period. Then the baseline image (F₀) was subtracted from each image acquired to generate images that represent the relative change in fluorescent signal, ∆F-F₀ or ∆F. To visualize the fluorescence intensity changes during stimulation, ∆F signals during the stimulus period were averaged, scaled and encoded by color maps with red indicating an increase in signal intensity. The color maps were then superimposed onto the F₀ baseline grayscale image, in order to visualize the spatial fluorescence intensity changes in the afferent processes during stimulation.

To quantify changes in afferent calcium signals we analyzed the registered images in ImageJ. To quantify the signals in an entire afferent process innervating a neuromast, we applied an inclusive threshold to capture all the pixels within the process. The same threshold was applied to all wildtype and emx2 mutant processes. Each threshold was used to generate a ROI to compute mean intensity changes (∆F/F₀) within the entire process throughout the acquisition. To quantify afferent calcium signals per HC, circular ROIs with a diameter of ~3 μm (12 pixels with 268 nm per pixel) were placed on the afferent process beneath each HC within a neuromast. After creating these ROIs, we then computed and plotted the mean intensity changes (∆F/F₀) within each ROI during the acquisition period. Quantification of ∆F/F₀ magnitudes was performed using scripts written in Matlab (The Mathworks) as described previously (Hilliard et al., 2005). The signal magnitude was defined as the peak value of intensity change upon stimulation.

To quantify the colocalization between RibeyeB and nerve endings, the number of RibeyeB puncta that were contacted by a single-labeled neuron per HC were counted. To further quantify this, a Mander’s colocalization analysis between RibeyeB and tdTomato-positive nerve endings was conducted by first placing 6.5 μm² ROIs beneath each HC innervated by a single labeled-afferent neuron and the area of overlap was measured. These measurements were made on selected 1µm optical sections centered on the ribbons to avoid overlap with the tdTomato-positive nerve fiber in different planes. Then, the Mander's coefficient was calculated using ImageJ. These values were averaged to determine the amount of overlap per neuromast. To quantify the number of RibeyeB and Maguk puncta, we used ImageJ to z-project all planes containing synapses. Then, we used ImageJ to apply the same background subtraction and threshold to each immunostain. After this processing we counted the total number of puncta, as well as complete and incomplete synapses by eye. For these counts, images were scored blinded. For RibeyeB and Maguk colocalization, we calculated the Mander’s coefficient to determine the amount of Maguk label that colocalized with Ribeye label, due to the high background in Maguk immunostain.

For our figures, images were processed and adjusted for brightness and contrast with ImageJ. Graphs were generated by Prism. Figures were assembled with Adobe Photoshop CS5.

To compare the afferent calcium signals per HC, a Kruskal-Wallis test in Prism was used. To compare the average afferent calcium signal per afferent process, number of spikes a one-way ANOVA in Prism was used. To compare complete and incomplete synapses, colocalization coefficients and number of innervated HCs between wildtype, emx2 ko and emx2 gof, a one-way ANOVA in excel was used. To compare the number of innervated HCs or Emx2-positive HCs between WT and vangl2^m209 mutants, a student’s t-test was used. In all graphs, errors bars represent standard error of the mean (SEM).

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

We would like to thank Alisha Beirl for technical assistance, Jennifer Wang for quantification of RibeyeB and Maguk staining, Dr. Lopez-Schier for the HGn39D strain and ZIRC for the vangl2^m209 strain. We are also grateful to Drs. Lisa Cunningham and Thomas Friedman and members of our laboratories for critical reading of the manuscript. This study is supported by NIDCD Intramural program awards to DKW and KK.

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