Brain connectivity maps display a delicate balance between individual variation and stereotypy, suggesting the existence of dedicated mechanisms that simultaneously permit and limit individual variation. We show that during the development of the Drosophila central nervous system, mutual inhibition among groups of neighboring postmitotic neurons during development regulates the robustness of axon target choice in a nondeterministic neuronal circuit. Specifically, neighboring postmitotic neurons communicate through Notch signaling during axonal targeting, to ensure balanced alternative axon target choices without a corresponding change in cell fate. Loss of Notch in postmitotic neurons modulates an axon's target choice. However, because neighboring axons respond by choosing the complementary target, the stereotyped connectivity pattern is preserved. In contrast, loss of Notch in clones of neighboring postmitotic neurons results in erroneous coinnervation by multiple axons. Our observations establish mutual inhibition of axonal target choice as a robustness mechanism for brain wiring and unveil a novel cell fate independent function for canonical Notch signaling.https://doi.org/10.7554/eLife.00337.001
The brains of all members of a species are similar, but not identical, and these differences are partly responsible for the range of behaviors displayed by individuals. The development of the nervous system is known to depend on the Notch signaling pathway, but the mechanisms that regulate the balance between fixed patterns of neuronal connectivity vs individual variability are largely unknown.
Notch proteins are transmembrane proteins, which means that they have one part inside the cell membrane and another outside the cell. When a ligand protein—such as a Delta ligand—binds to the part that is outside the cell, the Notch protein breaks in two and the part inside the cell travels to the nucleus, where it can influence the expression of genes.
Cells are selected to become neurons through a process known as mutual, or lateral, inhibition. When a Delta ligand belonging to one cell binds to the Notch receptor on a neighboring cell, the production of Delta ligands in the second cell is reduced. This amplifies any initial differences in the amount of Delta produced by each cell, and leads ultimately to them becoming distinct cell types.
Now, Langen et al. show that this same mechanism is reactivated at a later stage of development during wiring up of the visual system. They used the fruit fly (Drosophila)—a model organism with a fully sequenced genome and short intergeneration time—to study a group of brain cells known as dorsal cluster neurons. At the end of the fruit fly larval stage, these neurons extend long axons across the brain to the opposite hemisphere: however, it is unclear how the neurons decide which cells to form connections with.
Using genetically modified flies, Langen et al. showed that inhibiting Notch in a single dorsal cluster neuron caused that neuron to target a different cell: however, other neurons adjusted their choices accordingly so that the overall pattern of connections remained unchanged. Inhibiting Notch in a cluster of dorsal cluster neurons, on the other hand, disrupted the entire network, suggesting that Notch-mediated communication between neurons (via mutual inhibition) is needed to establish a robust wiring map.
Langen et al. suggest that evolution has favored a mechanism that ensures that the overall pattern of connections within a circuit is preserved, while individual connections differ from one species member to the next.https://doi.org/10.7554/eLife.00337.002
Conceptually, coupling axonal target choice to neuronal cell fate determination has the advantage of generating highly reproducible wiring patterns. However, it has the evolutionary disadvantage of limiting individual variability, and thus efficient adaptation to environmental change. Furthermore, a strictly deterministic coupling has the significant developmental disadvantage of limiting cellular plasticity in response to inevitable genetic and epigenetic variability within the developing brain (Muotri et al., 2005, 2010). The latter point is particularly critical in neuronal lineages that are intrinsically variable in cell number.
Notch signaling is a highly conserved crucial regulator of early nervous system development. The most well-established function for Notch signaling in neural development is the selection of neural progenitor cells through a process termed mutual or lateral inhibition (Artavanis-Tsakonas et al., 1999). In lateral inhibition, a group of equivalent neuroepithelial cells that initially express roughly the same Notch activity are eventually segregated in two groups defined by expression and activity levels of the receptor Notch and its membrane-bound ligand Delta. Due to cell–cell communication among overlapping clusters of adjacent cells, small differences in Notch expression level are amplified. As a consequence, the majority of cells within these clusters express high Notch activity levels, whereas a minority of cells express low Notch activity. These cells then go on to differentiate as neuronal progenitors. A second important function for Notch signaling is the establishment of alternate binary cell fates of sibling neurons. In contrast to lateral inhibition, this function requires the asymmetric inheritance of the Notch antagonist Numb by one of the two sibling neurons in a terminal cell division (Guo et al., 1996; Spana and Doe, 1996; Knoblich, 1997). It has been proposed that early binary cell fate specification via Notch-Delta signaling results in alternative axon targeting. In the fly visual system, the R7 and R8 photoreceptors, which independently require Notch activity to be specified, make alternative axonal target choices that appear to be consequences of their different fates. Indeed, their canonical fate marker transcription factors Prospero and Senseless, respectively, are required for this differential targeting (Morey et al., 2008). In the olfactory system of Drosophila, sibling neurons target their axon to different central nervous system (CNS) glomeruli due to differential cell fate specification (Endo et al., 2007). A recent elegant extension of this work shows that chromatin modification of Notch targets by the Hamlet protein further diversifies cell fate and axonal targeting in olfactory neurons (Endo et al., 2012). Interestingly, in this work, the effects were not restricted to sibling neurons, but extended to neighboring non-sibling neurons, and the corresponding effects on axonal targeting were not strictly binary nor fully penetrant leading to speculation that Notch activity might have probabilistic effects on axonal targeting downstream of cell fate specification (Schmucker and Hassan, 2012). Finally, an extensive analysis of CNS neurons in the fly olfactory circuit shows that there are more diverse wiring morphologies than can be accounted for by the number of cell types (Chou et al., 2010), suggesting that post-fate mechanisms may be crucial in wiring the Drosophila CNS. What these post-fate mechanisms are, and how they buffer intrinsic variability to generate stereotyped wiring patterns, is unknown.
Here we show that the dorsal cluster neurons (DCNs), a group of bilateral commissural higher order neurons in the visual system of Drosophila (Hassan et al., 2000) are intrinsically variable in number within and between individuals, yet generate a highly stereotyped wiring diagram. We combine high resolution quantitative anatomical analyses, computational modeling, and genetic dissection to show that Notch-mediated mutual inhibition acts late in development on postmitotic neurons to bias axonal target choice. Finally, we show that this mechanism ensures the reproducibility of the DCN connectivity pattern.
DCNs are produced from a single embryonic neuroblast, and all express the same cell fate markers, namely the Atonal (Hassan et al., 2000) and Acj6 (see below) transcription factors. All postmitotic DCNs are efficiently labeled with the ato-Gal4 driver starting at the third instar larval (L3) stage (Figure 1A). DCNs innervate two regions of the optic lobes, the lobula and the medulla. This binary axon target choice is a result of three distinct steps (Srahna et al., 2006). First, in late third instar larvae DCN axons grow en masse toward the developing medulla neuropil attracted by a Wnt5 signal. Second, at 25–50 hr after puparium formation (APF), most DCN axons begin to retract back to the lobula neuropil, likely in response to a repulsive fibroblast growth factor (FGF) signal (Figure 1A′–A″ ). Wnt and FGF have opposing effects on Jun N-terminal Kinase (JNK) activity, which is both necessary and sufficient for DCN axon growth. Third, a small subset of regularly spaced axons resist the repulsive signal, by an unknown mechanism, and remain in the medulla (Figure 1A′′′ ). These observations hint that the pattern of DCN axons may arise by a sorting mechanism that generates two mutually exclusive DCN axon target choices: lobula vs medulla (Figure 1B″).
To gain insight into how the two choices arise during DCN development, we carried out careful quantification of the number of DCN neurons and their axons in a cohort of genetically identical flies. Briefly, DCNs were labeled with GFP, driven by ato-Gal4, and imaged. Each DCN soma and axon were assigned 3D coordinates and analyzed with the ‘clusterdata' function in MATLAB (see the ‘Materials and methods' section for imaging and DCN profile details). These analyses reveal a number of interesting features. First, all DCNs express the same cell fate markers, Atonal and Acj6 (Figure 2A–B′), as detected by antibody staining, already at L3 prior to initiating axon outgrowth towards the optic lobes. Second, although there are on average 38 DCNs producing a highly stereotyped pattern of 12 spaced axons in the medulla (Figure 2C), the DCN lineage itself is not fixed. The number of neurons varies (35–43 neurons) not only between different individuals but also between the right and left sides of the same individual (r = −0.148; Figure 2D). Furthermore, there is no correlation between the number of neurons in a cluster and the number of medulla axons it projects (Figure 2—figure supplement 1, top graph). Thus, the DCNs represent an intrinsically variable lineage of similar neurons.
Next, we investigated whether positional information may play a role in determining medulla vs lobula target choice. DCNs are born in a ventral to dorsal order (Zheng et al., 2006), and each DCN establishes one ipsilateral dendritic arbor and one contralateral axonal arbor (Srahna et al., 2006; Nicolai et al., 2010). Using the flip-out technique (Wong et al., 2002), we labeled single DCNs with membrane-bound GFP and visualized them in the background of the entire cluster labeled with LacZ. We found that medulla targeting neurons are located all along the dorsal–ventral (D-V) and proximal–distal axes of the cluster (Figure 2E–G). Thus, there is no correlation between birth order and medulla vs lobula targeting, confirming earlier observations that sibling DCN clones generated using the MARCM technique can target the medulla, the lobula, or one each (Zheng et al., 2006). Interestingly, however, the D-V position of an axon is directly and very highly correlated (r = 0.964) with the D-V position of its soma within the cluster (Figure 2H and Figure 2—figure supplement 1, bottom graph) such that the most dorsal neuron gives rise to the most dorsal axon and so on (Figure 2H). Because most DCNs at any given D-V position innervate the lobula and a few innervate the medulla, D-V positional information does not directly instruct lobula vs medulla target choice.
We wondered whether cell–cell interactions might offer insight into the mechanism underlying the generation of a stereotyped medulla innervation pattern, despite variability in neuronal number. To this end, DCN soma were labeled with LacZ and their axons with CD8-GFP. Next, each neuron and each medulla axon were assigned their three-dimensional (3D) Cartesian coordinates (Figure 3A–D and Figure 3—figure supplement 1) to determine the distances between DCN cell bodies, and between each two adjacent medulla axons (see ‘Materials and methods'). These analyses reveal two features. First, DCN soma show a few sparse cells at the dorsal and ventral extremities and a majority of cells densely packed medially (Figure 3C,D). Second, DCN medulla axons are more dense dorsally and ventrally, but more sparse medially (Figure 3B). Therefore, there is an inverse correlation between cell density and interaxonal distance along the D-V axis in the medulla: four to eight medial DCN soma provide one medulla axon, whereas only one to two DCN soma target one axon to the medulla dorsally and ventrally (Figure 3E). It is crucial to note that this inverse relationship between soma density and medulla axon density is conserved in response to changes in cluster shape (Figure 3—figure supplement 2), yet the overall wiring pattern is preserved, strongly suggesting that DCNs use a dedicated mechanism to ensure the accuracy of the stereotyped medulla innervation pattern.
Together, the combination of data thus far suggests that the probability of any neuron targeting the medulla is independent of its absolute position in the cluster, but negatively dependent on the number of its neighboring neurons. One hypothesis to explain these observations stipulates the following: DCNs operate as several small overlapping subclusters in which all neurons within a certain distance of each other compete to provide one medulla axon (Figure 3F). In this model, neurons with fewer neighbors, as often seen dorsally and especially ventrally, target the medulla with higher probability. Conversely, densely clustered neurons, as seen medially, target the medulla with lower probability, and thus fewer axons. What genetic mechanism could underlie such a selection process?
Conceptually, the model above is similar to the generation of neural precursor cells from small subsets of interacting ectodermal cells, also known as proneural clusters. Notch-mediated mutual inhibition gives rise to a few regularly spaced single neural progenitors while the majority of cells adopt the alternative epidermal fate (Campos-Ortega and Jan, 1991; Artavanis-Tsakonas et al., 1999). Indeed, DCNs express Notch and its ligand Delta during the time when DCN axon sorting is occurring (∼32 hr APF; Figure 4A–A‴). At this stage, all DCNs also express the Delta regulator Neuralized (Neur) and the canonical Notch pathway transcriptional reporter E(spl)-CD2 (Bailey and Posakony, 1995; Lecourtois and Schweisguth, 1995; Lai et al., 2001; Pitsouli and Delidakis, 2005; Figure 4B–C). Strikingly, using anti-CD2 antibodies, we find differences in the levels of the Notch activity reporter among individual DCNs: most cells express relatively high levels of E(spl)-CD2, whereas a minority of cells scattered across the D-V axis of the cluster express relatively low levels (Figure 4D–F′). In contrast, E(spl)-CD2 levels are very low in DCNs at L3 (data not shown) suggesting that Notch signaling is not active in postmitotic DCNs prior to pupariation. Finally, we do not detect expression of the asymmetric inherited Notch inhibitor Numb in the DCNs nor a phenotype with numb RNAi expression (data not shown), suggesting that differences in Notch activity between DCNs are unlikely to arise by differential inheritance, a cell fate determinant. Together these data show that Notch signaling is active within the DCNs at the time of axon target sorting.
To examine the potential consequence of N-mediated mutual inhibition on an irregular 3D cluster of neurons, we first extended an existing computational model developed for mutual inhibition in a regular 2D hexagonal lattice (Collier et al., 1996) to quantitatively describe the emergence of DCN axon target choice from DCN cell clusters (see ‘Materials and methods' and Figure 5—figure supplements 1 and 2). The model predicts medulla targeting by a similar number and pattern of DCN axons as observed in vivo (Figure 5A red cells, Figure 5C). Next, as no previous modeling of Notch has been performed under loss of function conditions, we tested reduced Notch activity in silico. In this case, the model predicts that the stereotyped number and pattern of DCN medulla axons are disrupted. Specifically, the medulla is targeted by an increased number of axons (17.29 ± 3.96) arising from several small clusters (2–3) of neighboring neurons, especially medially (Figure 5B, red cells and blue arrows, Figure 5C).
To test these predictions, we asked whether Notch signaling is required within the DCNs. We used the ato-Gal4 driver to inhibit Notch and Delta specifically in postmitotic DCNs during adult brain development. It is critical to note that during adult brain development, ato-Gal4 is only active in DCNs postmitotically and after their axons begin to grow (Hassan et al., 2000; Srahna et al., 2006; Zheng et al., 2006). Postmitotic, DCN-specific inhibition of Notch or its ligands Delta and Serrate (Ser) leads to two phenotypes. First, we observe clustered axons at several D-V positions, particularly medially, as opposed to isolated single axons seen under control conditions (Figure 5D–F′,l) causing a significant decrease in axon–axon distances in the medulla (Figure 5K). Second, we observe a significant increase in the number of axons targeting the medulla (Figure 5L and Figure 5—figure supplement 3), indicating that axon clustering is the result of neighboring axons erroneously making similar target choices. These data quantitatively mirror the phenotypes predicted by computational modeling of mutual inhibition among DCNs. Importantly, loss of Notch function alters neither the number (38.13 ± 2 SD vs 37.12 ± 3.1 SD, Figure 5—figure supplement 4) nor the expression of DCN fate markers (Figure 5—figure supplement 5). RNAi knockdown of Neur, a positive regulator of Delta and Ser activity, causes clustered axons and a significant increase of medulla axons (Figure 5G,L). Finally, postmitotic and DCN-specific RNAi knockdown of the canonical Notch pathway nuclear effector proteins Suppressor of Hairless (Su(H)) and Mastermind (Mam) also result in axon clustering and a corresponding increase in medulla axon number (Figure 5H–J′,M). Altogether, these data support the notion that DCNs require Notch-mediated mutual inhibitory interactions to make accurate medulla vs lobula axon target choices.
Previous work has shown that high JNK activity is required for DCN axons to resist retraction and innervate the medulla. We hypothesized that N and JNK might interact negatively in neurons as described in Drosophila embryos and mammalian cell culture (Zecchini et al., 1999; Chu et al., 2002; MacKenzie et al., 2004; Mateos et al., 2007). Furthermore, it has been proposed that downregulation of the axon guidance molecule p21 activated kinease1 (Pak1) via canonical N signaling attenuates JNK activity (Mateos et al., 2007), making Drosophila Pak an attractive target candidate in our system. Indeed, we find that gain of Pak function, by expression of the constitutively active Pak using ato-Gal4, phenocopies Notch inhibition resulting in a significant increase and clustering of medulla axons, while knockdown of Pak levels reduces the number of medulla innervations (Figure 6A–D). Next, we examined the DCN medulla targeting pattern under conditions of inhibition of both N and JNK, which have opposite effects on medulla targeting. Simultaneous downregulation of JNK and N activities, using dominant negative transgenes driven by ato-Gal4, results in a phenotype similar to JNK inhibition alone (Figure 6D). This supports the notion that N activity antagonizes JNK signaling. Simultaneous reduction of both Notch activity and Pak levels, using Pak RNAi, results in a phenotype indistinguishable from Pak reduction alone (Figure 6D), supporting the notion that Pak acts downstream of Notch. Finally, DCN-specific gain of Pak and loss of JNK activity shows a reduced number of medulla axons, resembling loss of JNK (Figure 6D). These data support a model whereby N reduces JNK activity via inhibition of Pak function (Figure 6E). To test this model further, we asked if gain of Notch function affects JNK activity and Pak expression levels. To this end, we expressed the constitutively active intracellular domain of Notch (NICD) in DCNs and examined the levels of JNK reporter construct puckered-LacZ (puc-LacZ; Reed et al., 2001). We found a significant reduction of puc-LacZ levels in response to Notch activation (Figure 6F). Next, we transfected the Drosophila neuronal cell line DmBG2-c3 with NICD and assayed the effects on Pak and phospho-JNK (active JNK) levels. This resulted in a significant decrease in both Pak and pJNK levels, consistent with our in vivo observations (Figure 6G). Together, these data suggest that Notch activity sets the baseline JNK activity threshold which distinguishes medulla-targeting from lobula-targeting neurons (Figure 6E).
The data above suggest that Notch signaling is required to segregate axon target choices sometime between L3 and adult. To determine more precisely the timing of Notch requirement, we took advantage of the dominant nature of loss of Notch function and a temperature sensitive Notch mutant allele (Notchts). Flies were raised at either the permissive (18°C) or restrictive temperature (28°C) between 0 and 96 hr APF (Figure 7A,B). Reduction of Notch activity at the restrictive temperature results in clusters of neighboring axons in the medulla and a significant increase in the number of medulla axons (Figure 7A–E). Next, we raised flies at the permissive temperature and shifted them to the restrictive temperature for 24 hr intervals at different APF stages (Figure 7A,B). Decreasing Notch activity only alters axon target choice between 24 and 60 hr APF, but neither before nor after (Figure 7B,E). Importantly, inhibition of Notch function specifically within the DCNs only during pupal development, using a combination of ato-Gal4 and a temperature-sensitive Gal80 (McGuire et al., 2003), results in a very similar phenotype (Figure 7E′). Finally, gain of Notch function via DCN-specific expression of NICD or Su(H) strongly reduces the number of medulla axons found in the adult brain, but, importantly, does not inhibit their initial outgrowth into the medulla (Figure 7F–J), confirming that canonical Notch signaling specifically regulates the ability of axons to remain in the medulla after initial targeting. Altogether, these data mean that Notch signaling is required within the DCNs specifically to segregate axon target choice at pupal stage between 24 and 60 hr APF, but neither before nor after.
A mutual inhibition model for axonal target choices makes three specific predictions (Figure 8A). First, loss of Notch in a single neuron should autonomously bias the target choice of the mutant neuron. Second, the process should be robust such that a change of target choice by the Notch mutant neuron should be compensated for by a neighboring neuron. Thus, the total number and spacing of medulla axons should remain within wild-type range. In contrast, loss of Notch activity in subclusters of neighboring neurons result in multiple axons from the same subcluster innervating the medulla. We set out to systematically test these predictions.
First, we asked if Notch acts cell autonomously by generating GFP-labeled single cell clones mutant for Notch function using the MARCM technique (Lee and Luo, 1999). We generated two types of clones: clones in which Notch activity is inhibited only in postmitotic DCNs specifically after L3 using dominant negative Notch, and Notch-null clones in which Notch is completely absent from single cells from the time they are born. We found that whereas only 24% of the control clones target the medulla, approximately 60% of all Notch mutant clones—both null and DN—do so, with the most pronounced effect occurring medially (p<0.001 null, p<0.001 DN, Fisher's exact test) (Figure 8B–D). In contrast, as expected, medial Delta mutant clones favor targeting the lobula (Figure 8B′) with little or no effect on dorsal or ventral clones (data not shown). Therefore, Notch signaling levels autonomously regulate the axon target choice of individual DCNs. These data validate the first prediction of the mutual inhibition hypothesis.
To test the second prediction, we labeled the entire DCN pattern with the red fluorescent protein Cherry and generated single GFP-labeled Notch mutant cells in that background (Figure 8E). Analysis of the number, clustering, and spatial pattern of medulla axons in these clones show that the Notch mutant axon remains correctly spaced and the overall number and pattern of axons in the medulla is indistinguishable from control (Figure 8E′,F and Figure 8—figure supplement 1). Next, we analyzed 23 axon–axon distances representing 12 individual mutant clones and compared them to the distances observed in controls. We found that 87% (20/23) of the mutant axons are within the normal range, as expected if neighboring control neurons innervate the lobula (Figure 8G). Crucially, the biased medulla innervation caused by loss of Notch activity does not alter the D-V positional relationship between neuronal soma and axon; dorsal neurons still project dorsally, medial neurons project medially, and ventral neurons project ventrally (Figure 8B and Figure 8—figure supplement 2).
To test the third prediction, we designed a novel genetic combination to create adjacent cell clones independently of birth order. To this end, we generated flies in which Notch activity can be stochastically manipulated in sets of ‘green' (GFP-positive) postmitotic DCNs, while their ‘red' (Cherry-positive) neighbors remain wild type (see ‘Materials and methods' for genotype details) in order to inhibit Notch function during axonal targeting in potentially interacting DCN subclusters. As controls, subsets of adjacent wild-type DCNs were labeled with GFP without inhibition of Notch activity. Of 20 control clones, 18 (90%) gave rise to normal medulla innervation patterns (Figure 8H–H″) with no effect on the number of medulla axons (Figure 8J). In two clones (10%), we observed one example of two adject axons each. In contrast, when Notch is stochastically inactivated in subsets of postmitotic DCNs, two types of phenotypes are observed. First, in 55% of all clones (24/44), the overall pattern remains normal, even though the mutant axons themselves target the medulla. Second, in 45% of the clones (20/44), in addition to mutant axons targeting the medulla (Figure 8I′, white arrows), axon clustering is observed (p=0.0094 Fisher's exact test). Furthermore, the number of medulla axons is significantly increased, and the axon–axon distances within these clones is drastically reduced (Figure 8I–K and Figure 8—figure supplement 3), suggesting that in these cases interacting neurons of one subcluster have been targeted by the stochastic inhibition of Notch. These data validate the third prediction and strongly support the idea of Notch-mediated interactions among neighboring cells.
Previously, two deterministic models have been proposed to explain the requirement for Notch signaling in brain connectivity. First, binary sibling neuron fate specification by Notch—as opposed to mutual inhibition—has been proposed as a mechanism of fate-dependent targeting of sensory axons (Endo et al., 2007). Notch has also been suggested to act as an axon guidance molecule via a noncanonical pathway in fly embryos (Crowner et al., 2003). We show that higher order CNS neurons utilize mutual inhibition via Notch signaling to establish a robust wiring map. However, in contrast to the classical process of mutual inhibition, which specifies early progenitor cell fate, we demonstrate that mutual inhibition is reused in postmitotic DCN neurons. Three arguments support this interpretation. First, the decision to target the medulla neuropil of single cell Notch null mutant clone is probabilistic (∼60%) rather than absolute (100%) as would be expected for cell fate specification. Second, the requirement for Notch signaling in establishing the wiring diagram is restricted to 24–60 hr APF, and third, Notch signaling affects neither the lineage size nor the expression of different cell fate markers in the DCNs early in development. It should be noted that medulla vs lobula axon target choice can be viewed as a form of sub-fate choice. The important discovery here is that this ‘sub-fate' is not a cell-autonomous translation of birth order instructions, but is rather subject to regulation by the choices of neighboring cells. In that sense, it extends the timing and plasticity of the phase during which neurons can be said to acquire their ‘fate'.
Here, we report lateral inhibition as a novel mechanism for brain wiring. It is likely that the inhibitory interactions are taking place between the neuronal cell bodies, especially given the requirement for the nuclear factors Su(H) and Mam and the effects on the E(spl) transcriptional reporter. However, interactions between axons prior to or shortly after their defasciculation within the medulla cannot be formally ruled out. Axonal target choice resulting from mutual inhibition by neighboring postmitotic neurons is interesting, not only as a novel function for Notch signaling but also as an additional layer of regulation that complements, but is independent of, traditional axon guidance cues. While it may be sensible for sensory neurons to couple fate to targeting so that the same sensory information is carried by the same type of neuron in different animals, it is reasonable to speculate that a degree of circuit-level plasticity is a more useful strategy in higher order brain centers, where meaningful information is likely to be encoded at the network level and not by single cells. It would be interesting to test if other patterns of alternative target choices by similar neurons, such as retinal projections into the midbrain (Brown et al., 2000), mammalian ocular dominance columns (Crowley and Katz, 2002), or the wiring variability of Drosophila olfactory interneurons (Chou et al., 2010) utilize similar mechanisms. Finally, given the inevitable and significant genetic and environmental variability in the real world, it seems rather intuitive that a mechanism that ensures the reproducibility of the connectivity pattern of an entire circuit, would be evolutionarily favored over a mechanisms that would risk the population connectivity pattern in favor of attempting to generate the same connectivity of precisely the same cell.
Flies were raised at 25°C or 28°C, except for temporal Notch activity experiments for which flies were raised at 18°C and shifted to 28°C during pupation for a specific time window of either 24 hr or until eclosion. For MARCM, crosses were set up at 25°C. 2 to 4 days after egg laying, samples were heatshocked for 3 hr at 37°C and shifted back to 25°C until eclosion. Axonal pattern analysis was done on freshly eclosed adult flies.
The following flystrains were used:
Figure 1: (A–A‴) w/+;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/+;
Figure 2: (A–B′) w/+;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/+; (C, D) w/+;;atoGal4-14a,UAS-CD8::GFP/UASLacZ.NZ; (E–H) yw, hsFlp/w;Sp/+;UAS FRT CD2, y FRT mCD8::GFP/+;atoGal4-14a,UASLacZ/+;
Figure 3: w/+;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/UAS-RedStinger;
Figure 4: (A) w/+;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/+; (B) w ;+;atoGal4-14a,UAS-mCD8::GFP/neurlacZA101;; (C–F′) w;UAS-m-CD8::GFP/E(spl)mβ-CD2;atoGal4-14a,UAS-LacZ/+;
Figure 5: (D, K, L) w/+;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/+; (E, K, L) w/+;UAS-mCD8::GFP/UAS-NotchEC;atoGal4-14a,UAS-LacZ/+; (F, L) w/+;UAS-mCD8::GFP/UAS-Dde;atoGal4-14a,UAS-LacZ/+; (G, L) w/+;UAS-mCD8::GFP/Neur RNAi; atoGal4-14a,UAS-LacZ/+; (H, M) w/+;UAS-mCD8::GFP/Su(H) RNAi;atoGal4-14a,UAS-LacZ/+; (I, M) w/+;UAS-mCD8::GFP/Mam RNAi;atoGal4-14a,UAS-LacZ/+; (J, M) w/+;Mam RNAi /Su(H) RNAi;atoGal4-14a,UAS-LacZ/+; (L) w/ N RNAi;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/+; w;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/UAS-SerDN; w;UAS-mCD8::GFP/ UAS-Dde;atoGal4-14a,UAS-LacZ/UAS-SerDN;
Figure 6: (A, A′, D) w/+;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/+; (B, B′, D) ) w/+;UAS-mCD8::GFP/UAS-NotchEC;atoGal4-14a,UAS-LacZ/+; (C, C′, D) w/+;UAS-mCD8::GFP/UAS-Pakmyr;atoGal4-14a,UAS-LacZ/+; (D) w/+;UAS-mCD8::GFP/Pak RNAi;atoGal4-14a,UAS-LacZ/+; bsk DN/+;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/+; bsk DN/+;UAS-mCD8::GFP/ UAS-NotchEC;atoGal4-14a,UAS-LacZ/+; w/+; Pak RNAi/ UAS-NotchEC;atoGal4-14a,UAS-LacZ/+; bsk DN/+;UAS-mCD8::GFP/ UAS-Pakmyr;atoGal4-14a,UAS-LacZ/+; (F) w/+;UAS-mCD8::GFP/UAS-NotchIntra;atoGal4-14a,puc-LacZ/+; w/+;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/+; w/+;UAS-mCD8::GFP/UAS-NotchIntra;atoGal4-14a,UAS-LacZ/+;
Figure 7: (C–E) Nts/w; UAS-CD8::GFP/+;atoGal4-14a,UAS-LacZ/+; (E′) w/N RNAi;tubGal80ts/+;atoGal4-14a,UAS-mCD8::GFP/+; (F, G, J) w/+;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/+; (H, I, J) w;UAS-mCD8::GFP/UAS-NIntra;atoGal4-14a,UAS-LacZ/+; (J) w/+;UAS-mCD8::GFP/UAS Su(H);atoGal4-14a,UASLacZ/+;
Figure 8: (B–D) FRT19A/FRT19A,hsFlp,tub-Gal80;UAS- GFP,UAS-nLacZ/UAS-NotchEC;atoGal4-14a,UAS-mCD8::GFP/+; (B′) FRT19A/FRT19A,hsFlp,tub-Gal80;UAS- GFP,UAS-nLacZ/ UAS-Dde;atoGal4-14a,UAS-mCD8::GFP/+; (C) FRT19A/FRT19A, hsFlp, Gal80;UAS- GFP,UAS-nLacZ/+;atoGal4-14a,UAS-mCD8::GFP/+; (C, D) FRT19A,N55e11/FRT 19A, hsFlp,tub-Gal80;UAS- GFP,UAS-nLacZ/+;atoGal4-14a,UAS-mCD8::GFP/+; (E–G) FRT19A/FRT19A, hsFlp,tub-Gal80;UAS- GFP,UAS-nLacZ/UAS-NEC;atoGal4-14a,UAS-mCD8::GFP/atoLexA,LexAop-TLNΔCherry; (H–H″, J, K) act5C >y >Gal4,UAS-mCD8::GFP/+;;atoLexA,LexAop-TLNΔCherry/LexAopFlp(N3); (I–I″, J, K) act5C>y>Gal4,UAS-mCD8::GFP/+;UAS-NotchEC/+;atoLexA,LexAop-TLNΔCherry/LexAopFlp(N3);
Figure 2—figure supplement 1: (top) w/+;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/UAS-RedStinger; (bottom) yw, hsFlp/w;Sp/+;UAS FRT CD2, y FRT mCD8::GFP/+;atoGal4-14a,UASLacZ/+;
Figure 3—figure supplement 1: w/+; +;atoGal4-14a,UAS-GFP,UAS-RedStinger/+;
Figure 3—figure supplement 2: (top) w/+; +;atoGal4-14a,UAS-GFP,UAS-RedStinger/+; (bottom) w/+;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/UAS-RedStinger;
Figure 5—figure supplement 3: Dicer2/w; UAS-mCD8::GFP/+; atoGal4-14a,UAS-LacZ/+; Dicer2/w; UAS-mCD8::GFP/Delta ds RNAi; atoGal4-14a,UAS-LacZ/+;
Figure 5—figure supplement 4: w/+;UAS-mCD8::GFP/+;atoGal4-14a,UAS-LacZ/UAS-RedStinger; w/+;UAS-mCD8::GFP/UAS-NotchEC;atoGal4-14a,UAS-LacZ/UAS-RedStinger;
Figure 5—figure supplement 5: w/+;UAS-mCD8::GFP/UAS-NotchEC;atoGal4-14a,UAS-LacZ/+;
Figure 8—figure supplement 1: FRT19A/FRT19A, hsFlp,tub-Gal80;UAS- GFP,UAS-nLacZ/+;atoGal4-14a,UAS-mCD8::GFP/atoLexA,LexAop-TLNΔCherry; FRT19A/FRT19A, hsFlp,tub-Gal80;UAS- GFP,UAS-nLacZ/UAS-NEC;atoGal4-14a,UAS-mCD8::GFP/atoLexA,LexAop-TLNΔCherry;
Figure 8—figure supplement 2: FRT19A/FRT19A, hsFlp,tub-Gal80;UAS- GFP,UAS-nLacZ/UAS-NEC;atoGal4-14a,UAS-mCD8::GFP/atoLexA,LexAop-TLNΔCherry;
Figure 8—figure supplement 3: act5C>y>Gal4,UAS-mCD8::GFP/+;UAS-NotchEC/+;atoLexA,LexAop-TLNΔCherry/LexAopFlp(N3);
Dissected larval, pupal, or adult brains were stained with specific primary antibodies using the protocol described (Hassan et al., 2000) and incubated with Alexa fluorescent secondary antibodies. Pictures from Drosophila brains were taken using confocal microscopy Nikon AIR confocal unit mounted on a TI2000 inverted microscope (Nikon Corp., Tokyo, Japan).
The following antibodies and dilutions were used: mouse anti-ACJ6 (1:10), rabbit anti-Ato (1:2000), mouse anti-Delta (1:20), rabbit anti-Notch (1:1000), rabbit anti-Numb (1:200), rabbit anti-DsRed (1:500), rabbit anti-GFP (1:1000), mouse anti-GFP (1:1000), mouse anti-LacZ (1:1000), mouse anti-NC82 (1:100), rat anti-nCadherin (1:20), and mouse anti-CD2 (1:5000).
Drosophila brains were imaged using confocal microscopy Nikon AIR confocal unit mounted on a TI2000 inverted microscope (Nikon Corp.). The Nikon microscope was equipped with a Plan Apo 20× (0.72 NA) and a Plan Apo60× oil immersion (NA 1.40) objective lens. ImageJ was used to create Z-projections from confocal stacks. Images such as single or merged figures were created using Photoshop. For ease of viewing, images were rotated so that the DCN cluster is located on the top left corner of every image. To analyze the expression pattern of the E(spl)-CD2 carefully within the DCNs, DCN soma were isolated from the background using ImageJ. Confocal sections revealing individual DCN soma were obtained and CD2 fluorescence intensity within the different DCNs was analyzed.
Data were presented as mean ± SEM. Results were analyzed using either Bonferroni or Kruskal–Wallis depending whether samples were normal distributed (Komogorov–Smirnoff test). In case of a single comparison, the Student's t-test or the Mann–Whitney test was used depending on the result of the normality test. Fisher's exact test was used for cases of contingency tables. For all statistical tests, GraphPad Prism was used.
To generate profiles of DCN soma and their medulla axons, each object of interest, neuron or axon, was tagged with a 3D coordinate (proximal–distal, dorsal–ventral, anterior–posterior axis) scanning through a stack of confocal sections using ImageJ-Cell Counter module (Figure 3—figure supplement 1). The 3D coordinates were eventually normalized according to cluster diameter or lobula length and saved as DCN profiles. While analyzing the confocal sections, the number of neurons and medulla innervations were counted as they are a result of the number of coordinates. To calculate neuron to medulla axon ratio, the medulla axon profile was divided into 10 regions with the ‘clusterdata' function in MATLAB. The size of each of the 10 units depends on the axonal pattern as determined by the cluster algorithm. The same division is then projected onto the soma cluster that generated the particular axonal pattern, to obtain 10 identical DCN soma divisions.
The computational model is implemented according to Collier et al. (1996) and is described below in detail.
The first function describes Notch activity of a cell over time. Notch activity of each cell is positively influenced by Delta activity in the adjacent cells. The second equation defines the intracellular level of Delta, which is influenced by Notch activity within the same cell. The third function computes Delta activity of adjacent cells. N and Delta represent Notch and Delta activity in each cell, whereas dl refers to the average Delta activity calculated based on adjacent cells. Notch and Delta activity are computed by functions parameterized by a, b, k, and h. The production rates are symbolized by the variables pn and pd, whereas μ and ρ represent decay rates.
In our simulation, we set the parameters to compute the differential equations described above as follows: a = 0.01, b = 100, k = 2, h = 2, μ = 1, ρ = 1, and pd = 1. pn depended on the signal strength of Notch signaling.
Initially Notch and Delta activity levels were set to its signal strength, which were either 100% to simulate control condition or 10% to resemble downregulation of the transgene of interest. We assumed that 10% in case of a reduced Notch activity level will reflect the in vivo condition best (in vivo 18.4 ± 2.22 SD vs in silico 17.29 ± 3.96 SD) since NotchDN transgene for example is a strong repressor of Notch activity. We also tested in silico downregulation of Notch to 30%, and this results in approximately 20.33 ± 6.91 SD medulla axons. Given that NotchDN is a strong repressor of Notch function, 10% was chosen to simulate an in vivo loss of Notch function. Additionally, a noise term of 0–1% was introduced to the initial settings of Notch and Delta signaling.
To determine the trans-Delta expression level of each DCN soma, all adjacent cells needed to be identified. Since Collier et al. (1996) used cells arranged in a hexagonal lattice, each cell had at most six adjacent cells, thus creating a subcluster of maximal seven cells. The DCN cluster consists of ∼40 DCN soma, which are arranged in three dimensions. To divide the DCN cluster in subclusters of an average size of seven cells, Euclidean 3D distances between DCN soma were examined. DCNs were split into subclusters of about seven cells when we applied an Euclidean 3D distance of 0.17 [nad] (=normalized arbritrary distance) (Figure 5—figure supplement 2). Additionally, this also resulted in approximately 12 medulla axons (Figure 5—figure supplement 3).
To solve the differential equations described above, the Runge–Kutta (2, 3) formula was used for a timespan of 1000 time steps. During each timestep, each DCN soma was updated in its Notch and Delta expression level in three steps. First, ‘trans-Delta' expression was determined. For this, Delta expression of adjacent DCN soma was detected using 0.17 [nad] as an Euclidean distance.
Second, Notch activity level of a given DCN was updated based on the average Delta expression in adjacent cells. Finally, Delta expression of a given DCN is recalculated based on Notch activity in that cell. These calculations were performed for each DCN soma and repeated a 1000 times.
After solving the different equations, the final Notch expression level of each cell was analyzed. For each subcluster, the DCN soma with the lowest Notch activity was determined since these DCN soma will project its axon toward the medulla. Under wild-type conditions, each subcluster has on average only one DCN soma with the lowest Notch activity, whereas under loss of Notch signaling, multiple DCN soma are predicted to have equally low Notch activity levels. Matlab Version 188.8.131.524 (R2008a) was used for computational simulations and predictions.
The mathematical model is applied to analyze different aspects of the DCNs. First, the mathematical model should predict under control and loss of Notch activity condition the number of medulla axons to a certain degree. For this purpose, 16 different in vivo DCN clusters with their normalized 3D coordinates were taken as input for the mathematical model. These 16 DCN clusters were simulated a 1000 times. From these resulting 1600 data points, the average number of medulla axons, the standard deviation, and the standard error of the mean were calculated. Second, to analyze the final Notch activity pattern within an in vivo DCN cluster simulating either the control or loss of Notch condition, a single DCN cluster was applied to the mathematical model and presented in a 3D chart using different colors to symbolize lobula vs medulla DCN neurons (Figure 5A,B).
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Andrea BrandReviewing Editor; University of Cambridge, United Kingdom
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 choosing to send your work entitled “Mutual inhibition among postmitotic neurons regulates robustness of brain wiring” for consideration at eLife. Your article has been evaluated by a Senior editor and 3 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 based on the reviewers' reports.
Langen et al describe a developmental mechanism of neural wiring in the Drosophila visual system in which antagonistic interactions, via Notch signaling, in post-mitotic neurons, define distinct axon target choices within a lineage of apparently identical neurons. This is an interesting finding, which is globally well supported by the data, and which reveals a novel non-deterministic strategy by which reproducible nervous system connectivity is achieved.
The paper investigates how a single cluster of ∼38 neurons generated from a single neuroblast, and apparently molecularly identical, can still manage to have dramatically different projection patterns. The Dorsal Cluster Neurons (DCN) can either project to the medulla or to the lobula.
Very careful quantification of the projections and cell bodies indicates that there is extensive variability in the number of DCN produced from the unique neuroblast, as well as variability in the number of clusters along the dorso-ventral axis, but surprisingly a light level of stereotypy in the total number of neurons that project to the medulla.
The investigators explain how this is possible through a re-utilization of the same pathway used in lateral inhibition during the formation of embryonic neuroblasts, also in Drosophila. This is surprising as this Notch pathway acts as a lateral inhibitor only in the early steps of neurogenesis during embryogenesis, while we are dealing here with post-embryonic neurogenesis. One would have therefore expected a mode of lateral interactions mediated by asymmetric division of cells and asymmetric distribution of Numb, as in bristle precursor cells. The authors therefore show that, from each of the clusters of DCNs, only a fixed number of neurons, inversely proportional to the size of the cluster, choose to target the medulla rather than the lobula. Therefore, we are dealing with an embryonic type of Notch function rather then a post-embryonic mode.
Points to address:
* The authors argue repeatedly that the Notch choice is independent of the fate of the two populations of cells. However, this is far from being demonstrated as only two molecular markers are shown to be identical (Acj6 and Ato). It would take a lot more work to demonstrate that these are one type of neuron with different projection patterns. In fact, it is highly likely that the two cell populations are different from one another since they project differently, target different neurons, and might have different neurotransmitters. How can the authors be sure that there are not in fact two subsets of DCN neurons and that Notch functions classically in fate determination? This should be discussed.
* The authors address when Notch is required, but it is unclear where Notch functions and this could be clarified either with new data or at least in the Discussion. Is the Delta/Notch signaling functioning in the axons themselves (is Notch detectable in this compartment), or within the soma as implied indirectly by the relationship established early in the manuscript between DCN soma clustering and axonal target choice?
* The modeling is nice and does not detract from the quality of the paper. However, it is not necessary to use equations to predict that loss of Notch will lead to an increase in the proportion of medulla projecting neurons. Anyone who knows Notch would have predicted this.
* One reason for nature choosing to use the lateral inhibition system of the embryonic neurogenesis rather than the N on/N off Numb-biased choice might simply be the goal to achieve: in one case, a few neuroepithelial cells in the embryo decide to become neuroblasts while the majority remains epithelial (a case similar to the DCNs where the majority of neurons retracts to the lamina). In contrast, the Numb-mediated Notch function leads to 50-50 neurons A vs neuron B. In both cases, the neurons are different and it is likely that it is the same thing for DCN. Because the choice is made late, the common “master control” transcription factors establishing the lineage remain on late. But it is likely that a profiling of medulla vs lobula DCN neurons would lead to significant profile differences.
* Figure 8 contains several issues: for example, Figure 8h, it would be more illustrative to show an example in which a similar number of axons are labelled with GFP as in Figure 8i, because they claim that in the experimental condition the mutant (green) axons innervate the medulla, unlike the case in the control; but, because the control they show labels all the axons in green, it makes it difficult to appreciate the result, and prove that the effect is not solely due to the genetic flip-out manipulation in the neurons, but rather specifically due to the lack of Notch.
Figure 8i shows a cluster of one mutant (green) and one wild-type (red) axon, which is counter to their model that wild type axons compensate for the presence of mutant axons by restricting to the lobula – what is the explanation for this? Figure 8k: the distances between adjacent axons should be calculated for all axons and not only for GFP positive axons.https://doi.org/10.7554/eLife.00337.022
- Bassem Hassan
- Dietmar Schmucker
- Bassem Hassan
- Dietmar Schmucker
- Yves Moreau
- Bassem Hassan
- Marta Koch
- Dietmar Schmucker
- Yves Moreau
- Bassem Hassan
- Dietmar Schmucker
- Marta Koch
- Bassem Hassan
- Barret D Pfeiffer
The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.
We thank Gerald M Rubin for providing the unpublished LexAop-Flp lines, Utpal Banerjee for E(spl)-CD2 flies, Francois Schweisguth for Delta and neur RNAi flies, Jürgen Knoblich for the Numb antibodies, the Bloomington Stock Center and VDRC for Drosophila Stocks. We thank KU Leuven for providing the Software (Matlab) and Hardware that enabled computational analyses. We are very grateful to Sebastian Munck and the LiMoNe imaging facility for help with confocal microscopy. Confocal imaging was made possible through a Hercules Type 1 AKUL/09/037 grant coordinated by Wim Annaert. We thank Patrik Verstreken, Carmen Ruiz de Almodovar, and Ana Martin-Villalba for comments on the manuscript as well as Pierre Vanderhaeghen and members of the Hassan lab for stimulating discussions.
- Andrea Brand, Reviewing Editor, University of Cambridge, United Kingdom
- Received: October 24, 2012
- Accepted: January 22, 2013
- Version of Record published: March 5, 2013 (version 1)
© 2013, Langen 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.