Endogenous bioelectrical signaling coordinates cell behaviors toward correct anatomical outcomes. Lack of a model explaining spatialized dynamics of bioelectric states has hindered the understanding of the etiology of some birth defects and the development of predictive interventions. Nicotine, a known neuroteratogen, induces serious defects in brain patterning and learning. Our bio-realistic computational model explains nicotine’s effects via the disruption of endogenous bioelectrical gradients and predicts that exogenous HCN2 ion channels would restore the endogenous bioelectric prepatterns necessary for brain patterning. Voltage mapping in vivo confirms these predictions, and exogenous expression of the HCN2 ion channel rescues nicotine-exposed embryos, resulting in normal brain morphology and molecular marker expression, with near-normal learning capacity. By combining molecular embryology, electrophysiology, and computational modeling, we delineate a biophysical mechanism of developmental brain damage and its functional rescue.
Improper neural patterning during development leads to highly debilitating disorders, such as open neural tube defects [spina bifida, and anencephaly (small brain)]1, brain malformations2, and susceptibility to autism and degenerative disorders like Parkinson’s and Alzheimer’s diseases3,4,5. There are not currently any clinically approved interventions able to rescue such brain patterning disorders. Finding regenerative and repair strategies for brain patterning and function is a critical unmet need in developmental and regenerative medicine.
In addition to well-known growth factors and chemical pathways, endogenous bioelectrical signals (spatiotemporal distributions of resting membrane voltage—Vmem—across tissues) have been shown to regulate aspects of large-scale patterning during embryonic development6,7,8,9,10,11,12,13. Endogenous bioelectric signals (produced by the function of ion channels and pumps) have long been known to have roles in cell migration, wound healing, and the direction of growth and form in vivo14,15. Bioelectric signals are implicated in vertebrate appendage regeneration and development16,17,18, craniofacial morphogenesis19,20, left-right patterning21,22, cancer23, heart and muscle patterning24,25, planarian head regeneration26, and eye and brain patterning27,28. Here, we explore bioelectric signaling as both a target of teratogens that induce brain defects and as a target for therapeutic strategies to rescue such malformations.
Recent studies from our laboratory and other groups (reviewed in Ref. 15) identified molecular mechanisms by which bioelectrical signaling participates in development (including transduction machinery and transcriptional targets). However, the state-of-the-art for in vivo data in this exciting field has been “arrow diagrams” that identify the cellular-level bioelectric pathways of gene products and signals required for development or regeneration. The field still largely lacks knowledge of the quantitative dynamics that are sufficient to produce the spatial patterning across tissues or organs. Widely recognized as the next key step, but still missing, are biorealistic multi-scale models that integrate cell-level electrophysiology and molecular biology with large-scale patterning information (molecular, anatomical, and bioelectric). Such a synthesis is required in order to explain, in a rigorous manner, how bioelectric events originating with ion channel proteins scale up to regulate emergent organ patterning in health and disease. Here, we present and analyze the first example of such a model in the context of teratogenesis of the Xenopus brain and use it to identify a successful repair strategy.
Nicotine is a well-known neuroteratogen: embryonic exposure to nicotine leads to severe brain morphological defects as well as significant postnatal deficits in cognitive functions29,30,31,32. The majority of these effects of nicotine occur through its action on nicotinic acetyl choline (nAChR) receptors, but it is not known how this bioelectric change at the single-cell level alters whole organ morphogenesis of the brain. Here, we establish an amphibian model for nicotine teratogenesis, and exploit the Xenopus embryo as proof-of-principle of how computational models of physiological regulatory events can help identify mechanisms of developmental defects and drive the development of therapeutic strategies targeting endogenous bioelectricity.
Hyperpolarization-activated cyclic nucleotide-gated (HCN) channels are a group of voltage-gated ion channels in which the threshold voltage is modulated by the metabolic state of the cell (levels of cyclic nucleotides, like cAMP)33, thus allowing them to regulate cellular voltage in a context-specific manner. They open at hyperpolarized (negative) Vmem, giving rise to currents that are a mix of sodium and potassium fluxes. Among the four HCN isoforms (HCN1–4), HCN2 channels show an especially high sensitivity to cAMP. These channels are primarily present in the adult nervous system and heart, but have also been detected in human and mouse embryonic cells34,35,36,37. To the best of our knowledge, these channels have not been studied in the context of embryonic brain development or as targets for developmental therapeutics.
Here we present molecular physiology data and computational analysis explaining neuroteratogen nicotine-induced embryonic brain mispatterning. We report the first biorealistic computational model of Xenopus embryos, which predicts that nicotine disrupts the endogenous bioelectric patterns critical for brain patterning. This mispatterning mechanism is validated using voltage reporter dyes, and we model the consequences of possible methods for manipulating bioelectric gradients in vivo. Our model predicts that rescue would be effected by restoring this embryonic bioelectrical pattern via a reagent with context-specific effects on resting potential: the HCN2 channel. Remarkably, we find that misexpressing HCN2 channels in nicotine-exposed embryos rescues the endogenous spatial voltage gradient in the nascent neural tube and leads to a correction of the expression patterns of key brain transcription factors and a near complete rescue of brain morphology defects and cognitive learning abilities. Our integration of molecular developmental biology and simulation provides insight into the mechanisms of brain development and teratogenesis, and illustrates proof of principle of using computational modeling to understand and manipulate endogenous bioelectrical signaling in the context of regenerative medicine.
Embryonic nicotine exposure induces brain morphology defects
Nicotine is a well-known developmental neuroteratogen in humans29, causing morphological defects, decreased cognitive functions, and deficits in learning and memory. We first sought to establish a frog model of nicotine teratogenesis by exposing Xenopus embryos to nicotine (0.1 mg/mL). Nicotine exposure was targeted to stages 10–35, when neural tissue induction and patterning occurs. Untreated embryos served as controls, as neither ethanol nor dimethyl sulfoxide (DMSO) was needed to formulate the stock solution of nicotine used in our assays. Brain morphology of the embryos was assessed after they had developed to stage 45 (Fig. 1). Control tadpoles had correctly-patterned brain tissue5, with well-formed nostrils, olfactory bulbs/forebrain, midbrain, and hindbrain (Fig. 1a, d). Nicotine exposure caused a significantly high incidence of major brain morphology defects (~55%) in comparison to controls (~6%). The most striking phenotypes were the absence of nostrils, absence of forebrain, absence of both forebrain and midbrain, and occasionally misformed hindbrain (Fig. 1b, c) or truncated spinal cord. The hindbrain was the least affected of the brain regions. Eye development requires proper neural induction and development38,39. Tadpoles displayed abnormalies including missing eyes, incompletely formed eyes, fusion of eye to the brain, and pigmented optic nerves (Fig. 1b, c; see also ref. 27). We conclude that nicotine is a powerful neuroteratogen in Xenopus.
Model of V mem gradients patterning the embryonic brain
Our previous work demonstrated that specific Vmem distributions (pre-patterns) within the developing neural tube and surrounding regions are critical for proper patterning of the developing brain28, while other studies have characterized specific ion channels in developing of neuron populations40. No existing spatial model quantitatively synthesizes the functional and electrophysiological data to explain the control of patterning by endogenous ion channel activity; such a model is needed to understand the biophysics of organ development and to uncover mechanisms of action of ion channel-targeting teratogens. As bioelectric circuits can have highly non-obvious behavior, we used a computational platform, the BioElectric Tissue Simulation Engine (BETSE41), to characterize the dynamics of voltage gradients under the relevant conditions in vivo, and to develop a predictive physiological model (see Supplementary Note). BETSE is a software simulator specially designed to study bioelectricity from a “first principles” perspective, which focuses on ion concentrations, fluxes, and transport using realistic parameters derived from molecular physiology studies of cells to gain insight into spatialized dynamics of relevance to pattern formation41.
BETSE software was used to construct models of Vmem patterns in the early Xenopus neurula and to examine the influence of various interventions (Supplementary Note). Initial (i.e., simulation time zero) ion and substance concentrations in the cytosol, intercellular space, and global environmental media are summarized in Table 1. BETSE modeled an exterior sheet of cells representing an anterior view of a stage 15 Xenopus neurula, where cells were assumed to be a 10-μm-thick layer facing 0.1 × MMR (Fig. 2a). Voltage-sensitive gap junctions (GJs) were employed in all models, using the kinetic model of voltage sensitivity fit to amphibian gap junctions42.
A depiction of the complete bioelectric regulatory network underlying all BETSE models reported herein (including the optional elements: nicotine, IT, and HCN2 channels) is shown in Fig. 2b (Supplementary Note). The control model represents the fundamental (endogenous baseline) physiological situation, without nicotine treatment or IT misexpression. The control model considered three different spatial regions of cells, roughly demarcating the ectoderm, neural folds, and neural tube areas of the embryo from an anterior view of the outer surface (Fig. 2a). Variations in the base level of membrane permeability to K+ and Cl−(Fig. 2a) simulate the presence of leak channels, creating the observed endogenous relative hyperpolarization in the neural tube compared to the neural folds and ectoderm. This results in open Kir channels in the hyperpolarized neural tube region leading to a Vmem pattern of approximately −50 mV in the neural tube region, while the lateral neural folds and ectoderm remain at ~−5 mV (Fig. 3a, e). This hypothesis of generation of the endogenous Vmem pattern in the Xenopus neural tube is consistent with observed Vmem patterns in Xenopus embryos and the effect of dominant-negative Kir channels on them27,28.
Nicotine targets V mem prepattern to disrupt brain patterning
Simulation of nicotine exposure was built upon the control model by incorporation of nicotine-sensitive ionotropic nAChR receptors, expressed homogenously throughout the embryo43 (Supplementary Note). While nicotine is a well-known agonist of the nicotinic acetylcholine receptor (nAChR)44, it can also directly block a variety of K+ ion channels45, including the HCN channels46. Nicotine block of HCN channels is only partial (<39%). All this information was included in the models using a standard Hill function to describe the influence of nicotine on the channel state as a function of its concentration (Supplementary Note). Nicotine exposure simulated 0.62 mM diffusion of nicotine from the environment, which the model predicted would depolarize the Vmem by increasing Na+ membrane permeability (Fig. 3b, e). Treating the model with nicotine predicted to diminish the endogenous neural tube hyperpolarization pattern in comparison to controls (Fig. 3a, b, and e), thus reducing the spatial contrast of Vmem between the hyperpolarized neural tube and the depolarized neural folds and ectoderm (Fig. 3e). We tested the BETSE model predictions about nicotine effect on Vmem patterns in stage 15 embryos, using a combination of in vivo voltage reporter dye (CC2-DMPE:DiBAC4(3)) imaging47 and whole cell Vmem recordings27,28. Whole-cell electrophysiological recordings of Vmem from neural plate cells and flanking ectodermal cells provided calibration points for the voltage reporter dye images; the fluorescence intensities were analyzed against these calibration points to approximate membrane voltages at different points within the developing embryos (Fig. 4 and Supplementary Figure 1). Nicotine-treated embryos showed significant reduction in endogenous neural Vmem signal (depolarization by ~15 mV) in comparison to controls (Figs. 4a, b, e, f, and Supplementary Figure 1). This observation matches the BETSE model predictions of nicotine effect on Vmem both in direction (depolarization) and magnitude (~15 mV). Our model explains why nicotine induces brain defects: it correctly predicts the disruptive effects of this teratogen on the endogenous bioelectric prepattern required for brain development.
BETSE model identifies HCN2 channel as a repair reagent
Simulations of Vmem manipulation using an ion translocator (IT) involved the use of the control model with IT equally expressed in all cells. Simulations indicated that a homogenously expressed IT that opened preferentially in the hyperpolarized neural tube region, while remaining closed in the two lateral regions of the model, would lead to accentuation of neural tube Vmem pattern to ~−80 mV, while keeping remaining two regions of the model at ~−5 mV (Fig. 3c, e)—the spatial prepattern observed in wild-type embryos. The spatial patterning is crucial, as both depolarization of the middle region, or hyperpolarization of the lateral regions, both cause brain defects—it is the precise differential bioelectric state that induces the required balance of proliferation, apoptosis, and gene expression to build a normal brain28,48. Our model predicted that misexpression of an IT that amplified endogenous Vmem patterns (hyperpolarization) in the neural tube without affecting the Vmem patterns in the surrounding ectoderm would lead to maintenance of the endogenous neural tube Vmem pattern even in nicotine-exposed model embryos (Fig. 3c vs. d, e).
BETSE predicted HCN2 channels as an ideal reagent to meet this requirement. Its Vmem pattern amplification arises from the fundamental dynamics of the HCN2 channel in 0.1 × MMR (which is a low ionic environment). HCN2 channels (mostly studied in adult mammalian cardiac and neural tissues), in conjugation with voltage-gated Na+ and K+ channels, create self-oscillating Vmem signals33. The frequency of these Vmem oscillations is regulated by cAMP, which shifts the opening threshold of HCN2 channels to more positive Vmem values and couples HCN2-mediated Vmem oscillation frequency to cAMP modulators and cell metabolism33,49. Under Xenopus ionic parameters and external media, HCN2 channels hyperpolarize (Table 1 and Fig. 3f), which is also consistent with predictions using the GHK equation. HCN channels are primarily permeable to Na+ and K+ in a Na+:K+ ratio of ~0.2–0.33 (ref. 33). In this first model of the role of HCN2 channels in Xenopus development, the voltage and cAMP sensitivity of HCN2 channels were accounted for using kinetic models of HCN2 voltage sensitivity50 in combination with the assumption that the presence of cAMP shifts the V1/2 opening threshold of the HCN2 channel by + 20 mV (ref. 49) from its baseline value of V1/2 = 99.0 in the absence of cAMP50. HCN2 channel models used an Na+:K+ permeability ratio of 0.2 (ref. 33).
Our modeling predicted that HCN2 would be able to amplify the endogenous Vmem gradient patterns in Xenopus neurula (Fig. 3f). HCN2 channels are predicted to open at hyperpolarized Vmem, generating more hyperpolarization with opening, thereby serving as a Vmem-controlled switch of Vmem state, capable of amplifying small Vmem gradients, similar to IT effect (Fig. 3c, e, f). Thus, HCN2 channel transitions the Vmem of sufficiently electronegative cells to very hyperpolarized state, while leaving the Vmem of other relatively depolarized regions unchanged (Fig. 3c, e, f). Simulations indicated that homogenously expressed HCN2 channels open preferentially in the neural tube region, while remaining closed in the other two regions of the model. This leads to accentuation of neural tube Vmem pattern ~−80 mV, while keeping remaining two regions of the model at ~−5 mV, similar to IT (Fig. 3c, e, f). Importantly, our model predicts that HCN2 expression leads to maintenance of neural tube Vmem pattern even in nicotine-exposed model embryos, similar to the action of IT (Fig. 3c vs. d, e, f). This result suggests that HCN2 channels should amplify the intrinsic Vmem pattern of the neural tube, leading to a maintenance of Vmem pattern in spite of the depolarizing influence of nicotine. Thus, our computational model begins with a quantitative physiological explanation of the brain defects induced by nicotine and identifies an intervention strategy, predicting repair by the HCN2 channel.
HCN2 corrects V mem pattern in nicotine-exposed embryos
To test the predictions made by the BETSE model about nicotine’s and HCN2’s effects on membrane voltage prepatterns, we evaluated embryos between stage 15–17 using a combination of in vivo imaging with voltage reporter dye pair CC2-DMPE:DiBAC4(3) (ref. 47) and whole cell Vmem recordings (Fig. 4; refs. 27,28,]). Whole-cell electrophysiological recordings of Vmem from neural plate cells and flanking ectodermal cells were used as calibration points for the voltage reporter dye images, and the fluorescence intensities were analyzed against these calibration points to approximate membrane voltages at different points within the developing embryos (Fig. 4 and Supplementary Figure 1). Uninjected and untreated embryos (controls), embryos exposed to nicotine (stage 10 onward), embryos microinjected with Hcn2-WT (wild type) mRNA (both blastomeres at two-cell stage for an overall uniform expression) and embryos exposed to nicotine that are also injected with Hcn2-WT mRNA were analyzed.
Nicotine-treated embryos showed significant reduction in endogenous neural Vmem signal (depolarization by ~15 mV) in comparison to controls (Fig. 4a, b, e, f, and Supplementary Figure 1). This observation matches the BETSE model predictions of nicotine effect on Vmem both in direction (depolarization) and extent (~15 mV). Consistent with the BETSE model, voltage imaging in Hcn2-WT-injected embryos revealed a significantly enhanced endogenous neural signal (hyperpolarization by ~15 mV) in comparison to controls (Fig. 4a, c, e, f, and Supplementary Figure 1). However, the extent of enhanced hyperpolarization predicted by BETSE model for IT and HCN2 was higher (~30 mV) than actually observed (~15 mV) (Figs. 3e and 4). Crucially, nicotine-exposed embryos that were injected with Hcn2-WT channel mRNA showed remarkably enhanced (hyperpolarized better than controls by ~20 mV) endogenous neural Vmem signals in comparison to only nicotine treated embryos (hyperpolarized by ~30 mV) (Fig. 4a, b, d, e, f, and Supplementary Figure 1). This observation largely fits BETSE model predictions in both, direction of Vmem change, and extent of Vmem change (Fig. 3 and 4). As predicted, nicotine exposure suppresses the neural brain-specific Vmem pattern, while HCN2 channel expression enhances the neural Vmem pattern and restores it even in presence of the otherwise teratogenic nicotine. Having established that HCN2 can repair the bioelectric prepattern, we next assayed its effects on brain structure and function.
HCN2 overexpression reduces background brain defects
As a prelude to testing its repair function, we examined the effects of HCN2 channel expression on brain morphology and patterning in normal embryos. We injected Hcn2-WT mRNA into both blastomeres of wild-type embryos at the two-cell stage and assayed brain morphology at stage 45 (swimming tadpoles). Hcn2-WT mRNA injection increased the HCN2 channel levels by ~3.1 times (310%) in the injected embryos in comparison to controls as observed by immunostaining followed by quantitative analysis of control and injected embryos (Supplementary Figure 3). Even very small instances of morphological deviation from perfectly normal brain morphology were documented, including slightly shortened nostril distances, and unequal forebrain/olfactory bulbs. In untreated control embryos, a normal basal level of minor incidences of deviation from ideal brain morphology was observed in this very strict assay (~9%). Remarkably, we noticed that Hcn2-WT channel-injected embryos showed a significant reduction of these minor brain morphology phenotypes (~1.5%, **p < 0.01, t-test n = 3 with N > 50 embryos for each group for each of the experiments collected from multiple animals across independent clutches) (Fig. 5a, b): the channel mRNA-injected embryos were better than the controls. Thus, misexpression of HCN2 channels resulted in an improvement of developmental patterning even beyond that observed in control populations of unperturbed embryos raised under optimal conditions. This result is consistent with the use of our BETSE model to identify Vmem-modifying interventions that reinforce endogenous patterns and might be useful candidates for improving anatomical structure (Fig. 3c, e).
HCN2 rescues nicotine exposure-induced brain defects
To test the predicted effect of HCN2 on nicotine’s teratogenic influences on embryonic brain patterning, we exposed Xenopus embryos to nicotine (0.1 mg/mL – stage 10–35). We tested the effect of both Hcn2-WT and Hcn2-DN (dominant-negative) construct. Hcn2-DN was generated by mutating the highly conserved cation selective pore-domain GYG (amino acid 402–404) to AAA, a strategy known to drastically reduce conductance and generate dominant-negative mutants of HCN4 channels24,51 (Supplementary Figure 2). Hcn2-WT or Hcn2-DN mRNA was microinjected into both blastomeres at two-cell stage along with nicotine exposure. Untreated (uninjected) embryos served as controls. After the embryos were developed to stage 45, we quantified brain morphology (Fig. 5c–e). Control tadpoles had correctly patterned brain tissue5, including normally developed nostrils, olfactory bulbs, forebrain, midbrain, and hindbrain (Fig. 5c, f). As before (Fig. 1), nicotine exposure caused a significantly high incidence of major brain morphology defects (~60%) in comparison to controls (~7%) (Fig. 5c–f). Remarkably, Hcn2-WT mRNA-injected embryos showed a complete rescue of brain morphology defects from nicotine exposure, to levels (~6%) indistinguishable from that of untreated control embryos (~7%) (Fig. 5f). The nicotine-exposed, Hcn2-WT mRNA injected tadpoles showed nostrils, olfactory bulbs and forebrain, midbrain, and hindbrain that had formed similarly to controls (Fig. 5e). In contrast, nicotine-exposed embryos injected with a mutant, dominant-negative form of HCN2 failed to show rescue of brain morphology defects (~70%) (Fig. 5f).
To quantify brain shape, we used geometric morphometrics on stage 45 tadpoles52,53 (Fig. 6). Landmarks were chosen based on transition points between different brain regions, and lateral and anterior outermost points of the head (Fig. 6b) and recorded for n > 26 tadpoles for controls, nicotine, and nicotine + Hcn2-WT mRNA. Canonical variate analyses (Fig. 6a) were run on the data set, with Procrustes distances between each of the groups to characterize shape changes in each condition.
The quantification revealed whether the length of the brain was changed in relation to the head shape in nicotine-exposed embryos and whether Hcn2-WT mRNA injections restored wild-type proportions. Canonical variate analysis and Procrustes distances confirmed that control and nicotine + HCN2-WT group were not different in shape (Fig. 6a, green and red ellipses), but significantly different from nicotine-exposed embryos (blue ellipse) (Procrustes distances: Control vs. nicotine + HCN2-WT = 0.0446, Control vs. nicotine = 0.1222, and nicotine vs. nicotine + HCN2-WT = 0.1200). ANOVA of centroid shape between the controls and nicotine + HCN2-WT in relation to nicotine treatment confirmed significant differences between the groupings (F = 12.45, p < 0.0001). Thus, nicotine significantly changes brain shape, but Hcn2-WT mRNA microinjections restore brain morphology to the wild-type state.
HCN2 restores learning in nicotine-exposed larvae
Using an automated behavior analysis platform54,55 (Fig. 7a), a robust red-avoidance behavior can be produced and quantified in normal tadpoles (Fig. 7b, c). A tadpole was classified as ‘having learned’ if their preference for red light drops below 40% of time spent in red light, averaged across the final three probe sessions of the experiment. This approach has been successfully used to quantitatively evaluate brain function and learning performance under surgical, pharmacological, and genetic manipulations56,57,58. We tested nicotine-exposed tadpoles (0.1 mg/mL – stage 10–35) with or without the Hcn2-WT mRNA microinjection (0.75 ng/injection) in both blastomeres at two-cell stage.
Only ~12% (n = 26) of the nicotine-exposed tadpoles showed learning ability; the majority failed to learn in this automated behavioral test, in comparison to control tadpoles, which showed good learning abilities (100%, n = 25) (Fig. 7b, c, ANOVA p < 0.001), even though only the able-bodied (healthy, morphologically normal) nicotine-exposed animals were tested in this assay. As expected, the brain dysmorphias caused by nicotine were accompanied by severe performance defects. However, nicotine-exposed embryos receiving Hcn2-WT mRNA showed significant improvement in learning ability (85%, n = 20) in comparison to nicotine-exposed tadpoles (Fig. 7b, c, ANOVA, p < 0.001). Thus, HCN2 channels not only repair morphology, but also restore cognitive learning abilities in nicotine-exposed tadpoles.
HCN2 restores marker expression in nicotine-treated embryos
To determine the effects of HCN2 channel intervention in the hierarchy of known transcriptional regulators of brain patterning, we analyzed the expression of the key transcription factors otx2 (forebrain and midbrain), emx (telencephalon and forebrain), xbf1 (forebrain), and Pax6 (forebrain and eye)59,60,61,62.
Embryos with or without Hcn2-WT mRNA microinjection (both blastomeres at 2-cell stage) were exposed to nicotine from stage 10. Uninjected and untreated embryos were used as controls. Embryos were analyzed at stage 25 for expression of otx2, xbf1, emx, and pax6 by in situ hybridization (Fig. 8). The nicotine-exposed embryos showed significantly reduced expression of otx2 (in both area and intensity) and reduced or mispatterned expression of xbf1 in significant number of embryos [46% (χ2, p < 0.001) and 35% (χ2, p < 0.01), respectively] in comparison to control embryos (10% and 4.5%, respectively). In marked contrast, Hcn2-WT mRNA-injected embryos showed normal pattern of otx2 and xbf1 expression at similar levels to that of controls (4 and 4%, respectively). Nicotine exposure had little effect on emx and pax6 expression pattern, with minor reductions in a few embryos (17 and 12%, respectively) in comparison to controls (0 and 3%, respectively). Hcn2-WT-injected embryos exhibited normal emx and pax6 expression pattern at similar levels to controls (9 and 6%, respectively). Thus, HCN2 channel rescue of nicotine-induced defects includes correction of otx2 and xbf1, connecting HCN2-mediated repair of brain to the known molecular-genetic cascade of brain patterning factors.
Nicotine is a well−studied developmental neuroteratogen in humans29, non-human primates31, and invertebrates32. A fundamental gap in this area is the lack of mechanistic knowledge of how the effects on individual cell physiology result in impaired cognitive function. We addressed the developmental events that underlie the middle layer between cell behavior and organismal behavior—teratogenic effects of nicotine exposure on morphogenesis of the developing brain.
Bioelectric circuit9,10,11,63 dynamics are distinct from those of chemical gradients64,65,66 and are often complex. To bridge the gap between cell-level molecular electrophysiology and organism-level patterning and behavior, we used BETSE,41 a powerful and flexible biorealistic platform that enables predictions of bioelectrical patterns from channel expression and function data. We built a model of bioelectric patterns of neural stage Xenopus embryo, taking into account spatiotemporal dynamics of all different parameters including gap junctions, tight junctions, and relevant biochemical signals.
The endogenous early embryonic Vmem patterns across the neural tube are required for normal brain development28. Nicotine, an ion channel ligand, disrupts brain patterning (Fig. 1). We analyzed the BETSE model to understand how nicotine and IT actions would integrate at the level of embryonic Vmem patterning, and generate predictions and testable hypotheses.
Nicotine exposure diminished the endogenous neural tube hyperpolarization in the model (Fig. 3). Such disruptions in the brain specific Vmem pattern have already been shown to cause serious brain morphology defects28. In the model, HCN2 channels were seen to behave in a unique context-specific manner (Fig. 3f) that specifically amplifies the differential neural tube Vmem pattern across the neural plate despite the presence of nicotine (fitting the functional criteria of the model-derived IT). This predicts that context-specific action of HCN2 would strengthen the Vmem pattern otherwise diminished by nicotine and thus restores downstream transcription factors and brain patterning. Precisely, this was observed in our physiological profiling experiments (Fig. 4). It is also important to note that the model predicts that due to its context specific action, HCN2 channels also enhance the brain specific Vmem pattern of control (non-nicotine exposed) embryos (Fig. 3), consistent with our observation of patterning improvement of even the low incidence of brain defects in control batches of embryos (Fig. 5b). The BETSE model proved essential to quantitatively test this hypothesis and evaluate the properties of HCN2-containing circuits to reveal that they can indeed overcome the effects of nicotine on Vmem and do so appropriately depending on location in the neural tube center and its lateral areas. The balance of Vmem contrast between the neural tube and surrounding tissue has been shown to control the balance of proliferation and apoptosis in neural tube development48. This kind of sharpening of boundaries between distinct bioelectric compartments explains why HCN2 channels are able to correct even background brain defects (Figs. 5a, b).
An alternative case is where nicotine may directly affect endogenous HCN2 channels46, resulting in brain patterning defects. This suggests that normal endogenous HCN2 activity is required for proper brain patterning. However, our experiments with dominant-negative HCN2 channel shows that native HCN2 channel activity is not required for proper brain patterning (Supplementary Figure 4), thus negating this possibility. The effect of nicotine on the embryonic Vmem pre-pattern through nAChR (Figs. 2 and 3) is sufficient to explain the observed change in bioelectric state and the subsequent phenotypes, but our data do not rule out additional endogenous targets of nicotine. This is consistent with bioelectric mechanisms of action suggested for a number of other teratogenic chemicals67 and genetic syndromes68,69,70.
A critical next step for developmental physiology is to extend the understanding of single-cell electrophysiological properties (and ion channel expression) to spatialized dynamics that can explain the maintenance or disruption of large-scale patterns with relevance to developmental or regenerative patterning. To test predictions of the BETSE model, we generated Vmem maps of neurula stage Xenopus embryos under the different treatment conditions (Fig. 4). As predicted by the BETSE model, nicotine treatment indeed diminished the Vmem pattern (depolarized) by ~15 mV (peak Vmem in the neural tube) and HCN2 channel even in presence of nicotine increased the Vmem pattern (restored hyperpolarization) by ~35 mV (peak Vmem in the neural tube) (Figs. 3 and 4). In the case of HCN2 channel alone, the observed enhancement of Vmem pattern in relation to controls (~15 mV) was much less than the predicted value of increase by ~30 mV (Figs. 3 and 4). Since HCN2 channels are also regulated by cAMP and the context of cell metabolism, this difference may be the result of as yet unknown aspects of cell metabolism. It is also possible that there are other ion channels and pumps at play within the cells, affecting the action of HCN2 or directly influencing Vmem. We found an excellent quantitative match between the BETSE model’s predictions and the observed physiological and functional outcomes. To our knowledge, this is the first use of computational modeling to reveal spatialized bioelectric signaling dynamics that not only correctly predict the effects of a teratogen, but also show how to implement a rescue strategy.
Bioelectric interventions targeting ion flux have been used to induce regenerative response16,17. Here, we established a proof-of-principle extending this strategy to the use of ion channels as a reparative intervention for birth defects. Remarkably, HCN2 overexpression in embryos exposed to nicotine led to a complete rescue of nicotine-induced brain morphology defects (Fig. 5c–f). HCN2 channel overexpression restored not only gross brain morphology, but also the normal relation between brain length and the shape and size of the head (Fig. 6). This suggests that HCN2-mediated rescue involves sensing information from the surrounding regions to develop a brain with the correct size in relation to surrounding tissues and overall embryo proportions. Our prior work had pointed to the existence of a mechanism that coordinates brain sizing with remote tissue regions48. These consequences of HCN2 function are most likely due to its ability to act in a context-specific manner (Figs. 3 and 4)—it does not merely bring every cell to the same Vmem, but effects specific changes of resting potential that are different in distinct regions based on the local pre-existing Vmem. This ability to reinforce spatial differences enables embryos to establish the crucial embryonic brain-specific Vmem pre-pattern28,48 that is otherwise erased by nicotine exposure (Fig. 4).
A notable finding was the ability of HCN2 channels to improve the brain morphology of control embryos (Fig. 5a, b). This effect is likely also attributable to the context-specific actions of HCN2, which significantly enhance the crucial embryonic brain’s Vmem pre-pattern of these embryos (Figs. 3 and 4). These observations suggest that the restorative action of HCN2 is not limited to nicotine-induced brain morphology defects, but could reveal a more general mechanism of action, reinforcing the endogenous bioelectrical signals required for correct developmental brain morphology that might be partially destabilized by a wide range of exogenous teratogens or endogenous physiological/genetic lesions. The full scope of the kinds of defects that can be rescued by HCN2 remains to be delineated and is an active area of investigation in our laboratory.
We tested the effects of HCN2 on learning behavior in nicotine-exposed Xenopus embryos using an automated training apparatus54,55,56. Our data showed that HCN2 channels largely restore learning abilities in nicotine-exposed tadpoles (Fig. 7). This suggests that HCN2 along with restoring the physiological states necessary for normal brain morphology (Figs. 5 and 6) restores the internal wiring and networks necessary for normal learning abilities (Fig. 7). Given that HCN2 is able to fix learning abilities in addition to gross brain morphology, we suggest that HCN2 or other Vmem-based therapies could represent an important new direction for addressing learning and memory disorders that are related to such defects.
Endogenous Vmem patterns in neurula stage Xenopus embryos are critical for proper patterning and sculpting of brain tissue. Here we established an amphibian model for understanding nicotine neuroteratogenesis at the level of gene expression, electrophysiology, morphology, and behavior. Because of the central role of bioelectric circuits in normal brain development and teratogenesis, we formulated a predictive, biorealistic model of developmental physiology that explained the patterning of resting potentials across the neural tube under wild-type and disease conditions. Our model is the first quantitative explanation of teratogenesis targeting bioelectric controls of growth and form. Most importantly, it predicts that reagents that sharpen borders between bioelectric compartments will reinforce normal patterning, thus identifying a context-sensitive HCN2 ion channel as an intervention tool. We used HCN2 to confirm this prediction in vivo. Forced expression of HCN2 mRNA rescued nicotine-induced malformations, restoring not only the anatomy, but the gene expression in the nascent brain, and ultimately improving behavioral metrics of learning and memory. These data identify a patterning function that can be implemented using HCN2 in synthetic biology or in vivo. Taken together, our data shed light on a new mechanism of brain defects and establish proof-of-principle for using developmental physiology models to understand disorders of pattern and test interventions in silico. We provide a tool for predictive bioelectric modulation and demonstrate its use as a part of a tractable strategy for manipulating neurogenesis and neural patterning. Future work targeting native channels with small molecule compounds to effect rescue without gene therapy are currently on-going in our lab. Thus, activation or expression of specific channels is a general strategy for biomedical approaches to complex organ patterning in the context of birth defects, regenerative medicine, and bioengineering.
Xenopus laevis embryos were fertilized in vitro according to standard protocols71: in 0.1 × Marc’s Modified Ringer’s (MMR; 10 mM Na+, 0.2 mM K+, 10.5 mM Cl-, 0.2 mM Ca2+, pH 7.8). Xenopus embryos were housed at 14–18 °C (14 °C overnight after injection and subsequently at 18 °C), and staged according to Nieuwkoop and Faber72. We saw the normal very-low background levels of abnormal morphologies (<9%), indicating the good health of our animals and good rearing conditions. For animals used in behavior trials, individuals were raised under 12 h:12 h light:dark cycle at a temperature of 16 °C, at no more than 30 individuals per 100 × 25 mm Petri dish. After stage 46, tadpoles were fed twice per day on standard sera micron powdered food until behavioral testing. All experiments were approved by the Tufts University Animal Research Committee (M2017-53) in accordance with the guide for care and use of laboratory animals.
Capped synthetic mRNAs generated using mMessage mMachine kit (Ambion) were dissolved in nuclease free water and injected into embryos immersed in 3% Ficoll using standard methods71. Each injection delivered between 0.5–1 ng of mRNA (per blastomere) into the embryos, at the indicated stages into the middle of the cell in the animal pole. Hcn2-WT and Hcn2-DN were mammalian (mouse) (HCN) channel 2, modified as detailed in the supplemental documents.
Xenopus embryos were incubated in chemicals or pharmacological blockers dissolved in 0.1 × MMR during the stages of interest as indicated in respective experiments followed by several washes with 0.1 × MMR. The embryos were exposed (from stage 10 to 35 unless otherwise specified, because neural/brain tissue development takes place in this time period, allowing specific testing of effects on these processes while allowing cleavage and gastrulation to proceed normally) to the following: 0.1 mg/mL nicotine (Sigma). The dose of nicotine was titrated to a level at which no general toxicity was observed and survival rate of embryos was similar to untreated controls.
Tadpoles used for morphometric analysis were imaged with a Nikon SMZ1500 microscope with a Retiga 2000R camera and Q-capture imaging software. Landmark data were then recorded using ImageJ software73. Landmarks for morphometric analysis were chosen based on biological relevance and reproducibility across tadpoles with varying brain and head morphologies. Landmarks were: (1) anterior most tip of the head; (2) between the two olfactory bulbs at the beginning of the forebrain; (3) laterally center of the brain at the point of transition between forebrain and midbrain; (4) Laterally center of the brain at the point of transition between midbrain and hindbrain; (5) Transition point between hindbrain and spinal cord; and (6) and (7) Lateral outermost points of the head along the eyes. MorphoJ software74 was used for Canonical Variate Analysis, to quantify and graphically represent change in brain regions in relation to head shape. MorphoJ software was also used to calculate Procrustes distances and perform statistical analysis. Our analysis is conservative as nicotine-treated embryos that had major portions of their brain missing were not used since the same landmarks as controls could not be used (e.g., Fig. 1c). Only those tadpoles that had brain morphology defects, but still could be used to place the landmarks were used (e.g., Fig. 5d).
Associative learning behavior test
All behavioral trials were performed with a custom built automated training robot54,56. The device consists of an array of 12 individual chambers, each capable of holding a 60 × 15 mm petri dish filled 15 mls of 0.1 × MMR. Below each dish is a machine vision camera (Insight-Micro 1400, Cognex Corporation, Natick, MA, USA), which uses a background subtraction algorithm to track any animals in the chamber in a Cartesian manner. Illumination is provided to each chamber independently from above, by a control module capable of specifying color and intensity by quadrants within each chamber. Red or blue light is delivered by light-emitting diodes (Osram Semiconductors, blue LED; 470 nm part no. LBW5SM, red LED, 635 nm part no. LRG6SP) and Xenopus see both given the spectral profiles of their three known cone classes75. Each chamber also has a set of six, equidistant, iridium oxide-coated titanium electrodes allowing the delivery of mild to strong electric shocks. All shocks delivered during wavelength-mediated training experiments were 1.2 mA AC currents, pulsed for 100 ms followed by 300 ms of no shock. This value was previously determined to be the lowest that elicits a behavioral response and no animals displayed physiological or behavioral abnormalities upon completion of testing.
Tadpole color-based associative learning assay was performed as documented before56 (Fig. 7a). Individual tadpoles were introduced to the chamber, which was illuminated with half red and half blue light, in absence of any punishment to probe their innate color preferences. Innate testing lasted 30 mins with colors across quadrants inverted after 15 mins to avoid considering stationary tadpole as having a 100% preference for a particular color (if the tadpole is stationary inverting the color would result in 50/50 preference). Tadpole then enters learning acquisition phase where tadpole receives a 1.2 mA shock if it occupies the red quadrant. This duration is 20 mins, with colors in the chamber being inverted every 5 mins. Then tadpoles are given a 90 min rest period where the entire chamber is illuminated with blue light and no shock punishment is delivered. Finally, the tadpole is probed for learning of light preference by giving them a choice between red and blue light for 5 mins with no punishment. The entire block of acquisition-rest-probe is repeated 6 times.
All tadpoles used in behavioral trials were stage ~48. A tadpole was determined to have learned if their preference for red light was below 40%, averaged across the final 3 probe sessions of the experiment. Note, that tadpoles were fed directly before trials and small amount of food was added to each chamber during training, as hungry tadpoles fail to learn.
In situ hybridization
Xenopus embryos were collected and fixed in MEMFA (1 hour at room temperature)71 and in situ hybridization was performed as previously described71. Briefly, the embryos were washed with PBS 0.1% Tween 20 (PBST) and transferred through series of methanol washes 25–50% to 75–100%. In situ antisense probes were generated in vitro from linearized templates using a DIG-labeling mix (Roche). Chromogenic reaction times were optimized for signal-to-background ratio. Probes used were otx2 (ref. 76), xbf1, and emx (refs. 77,78). Antisense probe for Xenopus HCN2 was generated from X. laevis hcn2.L IMAGE clone 5514485 (Dharmacon): a HindIII fragment was deleted, leaving exons 2–4 and part of exon 5 as probe79.
Imaging Vmem using CC2-DMPE:DiBAC4(3)
CC2-DMPE and DiBAC4(3) voltage reporter dyes were obtained from Invitrogen and used as per the standard protocol, including dark-field and flat-field correction63. Briefly, the use of two dyes with opposite emission profiles simultaneously provides an internal control and allows ratiometric normalization. CC2-DMPE stock (5 mM) was dissolved 1:1000 in 0.1 × MMR and the embryos were incubated in the dark in this solution for at least 1 h followed by 5 washes with 0.1 × MMR. DiBAC4(3) stock (1.9 mM) was dissolved 1:1000 in 0.1 × MMR and the CC2-DMPE-stained embryos were then incubated in the dark in this solution for at least 30 min washed thoroughly in 0.1 × MMR, followed by visualization under the microscope. An Olympus BX-61 microscope equipped with a Hamamatsu ORCA AG CCD camera, and controlled by MetaMorph software (Molecular Devices), was used to collect signal. NIH ImageJ software was used to quantify the fluorescence intensities of the CC2-DMPE:DiBAC4(3) signal.
Intracellular recordings from embryo cells
Membrane potentials were measured using an oocyte clamp OC-725C amplifier (Warner Instruments) with a single voltage electrode. Microelectrodes were made from thin-walled borosilicate glass pulled with a flaming/brown micropipette puller (p-97; Sutter Instruments) and back-filled with electrode solution (2 M potassium acetate, 10 mM KCl, and 5 mM HEPES, pH 7.5). Tip resistances were 80–100 MΩ. Electrode penetration of ectodermal cells was by visual guidance on a fixed-stage microscope (Zeiss) using a three axis micromanipulator.
HCN2 channel detection was performed by immunofluorescence for HCN2 channel. Briefly, embryos were fixed overnight in MEMFA at 4 °C (ref. 71). The embryos were permeabilized in PBS 0.1% Triton X-100; blocked with 10% goat serum in PBST for 1 hour at room temperature; and incubated at 4 °C overnight with primary antibody (Anti-HCN2: ThermoFisher Scientific PA1-918) at 1:500 dilution in PBST + 10% goat serum (blocking buffer). Embryos were washed six times in PBST and incubated with Alexa Fluor-conjugated fluorescent secondary antibody (Invitrogen) at 1:500 dilution in PBST + 10% goat serum overnight at 4 °C. Sections were washed six times and photographed using an Olympus BX-61 microscope equipped with a Hamamatse ORCA AG CCD camera, and controlled by MetaMorph software. NIH ImageJ software was used to quantify the fluorescence intensities of the immunostained embryos.
A mouse HCN2 cDNA clone was kindly provided by Dr. Jeanne Nerbonne (Washington University). The HCN2 cDNA was cloned into the eukaryotic expression vector pcDNA3 (Thermo Fisher Scientific). To create the dominant-negative (DN) HCN2 mutation, the entire GYG signature motif in the channel pore was mutated to alanine-alanine-alanine (AAA) by site-directed mutagenesis. The forward primer was: 5’-ATGAGCCACATGC TGTGTATCGCCGCGGCACGACAAGCACCCGAGAGCATGACA-3’ and the reverse primer was: 5’-TGTCATGCTCTCGGGTGCTTGTCGTGCCGCGGCGATACA CAGCATGTGGCTCAT-3’. The WT or DN mutant of HCN2 was then sub-cloned into a bi-cistronic mammalian expression vector, pIRESGFP1 (kindly provided by Dr. David Johns, Johns Hopkins University), to create a CMVp-HCN2-IRES-eGFP fusion for subsequent studies. The HCN2 channel construct function was tested using voltage clamping in HEK293 cells (which do not have endogenous HCN channels) (Supplementary Fig. 2A).
Cell culture and transfection
HEK293 cells were cultured in Dulbecco’s Modified Eagle’s Medium supplemented with 10% fetal bovine serum, 100 μg/ml penicillin, and 100 μg/ml streptomycin in a 37 °C, 5% CO2, 95% air incubator as previously described (Makielski et al. 2003). Approximately 1 × 105 cells were seeded in a 35-mm-diameter culture dish containing 1.5-ml culture media. A volume of 0.7 µg DNA of HCN2-WT or HCN2-AAA or the empty vector control was transiently transfected into HEK293 cells at 80% confluency using a Fugene6 transfection kit (Roche Applied Science, Indianapolis, IN) following manufacturer’s instructions. The transfected cells were incubated at 37 °C for 24 h to allow protein expression.
Voltage clamp recordings
Whole-cell HCN2-encoded inward currents (IHCN) were recorded at room temperature from transfected HEK293 cells using voltage clamping as previously described (Ye et al. 2008; Ye and Nerbonne 2009). The extracellular solution contained in (mM): NaCl 110, MgCl2 0.5, KCl 30, CaCl2 1.8, and HEPES 5 while the pipette solution contained (in mM): NaCl 10, MgCl2 0.5, KCl 130, HEPES 5, and EGTA. The cells showing green fluorescence were identified under epifluorescence and selected for IHCN recordings. Recording electrodes were fabricated from borosilicate glass (WP Instruments) on a two stage (P-87; Sutter Instrument) vertical puller. IHCN was evoked in response to hyperpolarizing voltage steps to potentials between −60 and −130 mV from a holding potential of −40 mV. Data were collected using an Axopatch 200B amplifier interfaced to a Digidata1322A acquisition system (Molecular Devices, Sunnyvale, CA). Data were subsequently processed and analyzed using Axon pCLAMP10 Software Suite (Molecular Devices, Sunnyvale, CA). A one-way ANOVA with Bonferroni correction was carried out to determine the statistical significance between experimental groups. P < 0.05 was considered a significant difference between two groups.
All statistical analyses were performed using GraphPad Prism7. At least three independent experiments (n > 3) were conducted with N > 50 embryos for each treatment groups for each of those experiments collected from multiple animals across independent clutches. Data were analyzed by t-test (for two groups) or ANOVA (for more than two groups), as indicated with each experiment.
All data generated or analyzed during this study are included in this published article and its supplementary information files, or from the corresponding author upon request.
Copp, A. J. & Greene, N. D. Genetics and development of neural tube defects. J. Pathol. 220, 217–230 (2010).
Parrini, E., Conti, V., Dobyns, W. B. & Guerrini, R. Genetic basis of brain malformations. Mol. Syndromol. 7, 220–233 (2016).
Doganli, C., Beck, H. C., Ribera, A. B., Oxvig, C. & Lykke-Hartmann, K. alpha3Na+/K+-ATPase deficiency causes brain ventricle dilation and abrupt embryonic motility in zebrafish. J. Biol. Chem. 288, 8862–8874 (2013). M112.421529 [pii].
Goldman, S., O’Brien, L. M., Filipek, P. A., Rapin, I. & Herbert, M. R. Motor stereotypies and volumetric brain alterations in children with Autistic Disorder. Res. Autism Spectr. Disord. 7, 82–92 (2013).
Pratt, K. G. & Khakhalin, A. S. Modeling human neurodevelopmental disorders in the Xenopus tadpole: from mechanisms to therapeutic targets. Dis. Model Mech. 6, 1057–1065 (2013).
Nuccitelli, R. Endogenous electric fields in embryos during development, regeneration and wound healing. Radiat. Prot. Dosim. 106, 375–383 (2003).
Jaffe, L. F. Control of development by steady ionic currents. Fed. Proc. 40, 125–127 (1981).
McCaig, C. D., Rajnicek, A. M., Song, B. & Zhao, M. Controlling cell behavior electrically: current views and future potential. Physiol. Rev. 85, 943–978 (2005).
Levin, M. Molecular bioelectricity in developmental biology: New tools and recent discoveries: Control of cell behavior and pattern formation by transmembrane potential gradients. Bioessays, https://doi.org/10.1002/bies.201100136 (2012).
Levin, M. Endogenous bioelectrical networks store non-genetic patterning information during development and regeneration. J. Physiol. 592, 2295–2305 (2014).
Levin, M. Reprogramming cells and tissue patterning via bioelectrical pathways: molecular mechanisms and biomedical opportunities. Wiley Interdiscip. Rev. Syst. Biol. Med 5, 657–676 (2013).
Pai, V. P. et al. Genome-wide analysis reveals conserved transcriptional responses downstream of resting potential change in Xenopus embryos, axolotl regeneration, and human mesenchymal cell differentiation. Regen. (Oxf.) 3, 3–25 (2016).
Pai, V. P. & Levin, M. in Stem Cells: From Basic Research to Therapy, Vol. 1 (F. Calegari & C. Waskov eds) Ch. 5, 106-148 (Science Publisher, Taylor and Francis - CRC Press, Boca Raton, FL 2014).
Bates, E. Ion channels in development and cancer. Annu. Rev. Cell Dev. Biol. 31, 231–247 (2015).
Levin, M., Pezzulo, G. & Finkelstein, J. M. Endogenous bioelectric signaling networks: exploiting voltage gradients for control of growth and form. Annu. Rev. Biomed. Eng. 19, 353–387 (2017).
Adams, D. S., Masi, A. & Levin, M. H+pump-dependent changes in membrane voltage are an early mechanism necessary and sufficient to induce Xenopus tail regeneration. Development 134, 1323–1335 (2007).
Tseng, A. S., Beane, W. S., Lemire, J. M., Masi, A. & Levin, M. Induction of vertebrate regeneration by a transient sodium current. J. Neurosci. 30, 13192–13200 (2010).
Perathoner, S. et al. Bioelectric signaling regulates size in zebrafish fins. PLoS Genet. 10, e1004080 (2014).
Vandenberg, L. N., Morrie, R. D. & Adams, D. S. V-ATPase-dependent ectodermal voltage and pH regionalization are required for craniofacial morphogenesis. Dev. Dyn. 240, 1889–1904 (2011).
Adams, D. S. et al. Bioelectric signalling via potassium channels: a mechanism for craniofacial dysmorphogenesis in KCNJ2-associated Andersen-Tawil Syndrome. J. Physiol. 594, 3245–3270 (2016).
Aw, S. et al. The ATP-sensitive K(+)-channel (K(ATP)) controls early left-right patterning in Xenopus and chick embryos. Dev. Biol. 346, 39–53 (2010).
Levin, M., Thorlin, T., Robinson, K. R., Nogi, T. & Mercola, M. Asymmetries in H+/K+-ATPase and cell membrane potentials comprise a very early step in left-right patterning. Cell 111, 77–89 (2002).
Chernet, B. T. & Levin, M. Transmembrane voltage potential of somatic cells controls oncogene-mediated tumorigenesis at long-range. Oncotarget 5, 3287–3306 (2014).
Pitcairn, E. et al. Coordinating heart morphogenesis: a novel role for hyperpolarization-activated cycleic neucleotide-gated (HCN) channels during cardiogenesis in Xenopus laevis. Commun. Integr. Biol. 10, e1309488 (2017).
Lobikin, M., Pare, J. F., Kaplan, D. L. & Levin, M. Selective depolarization of transmembrane potential alters muscle patterning and muscle cell localization in Xenopus laevis embryos. Int. J. Dev. Biol. 59, 303–311 (2015).
Beane, W. S., Morokuma, J., Lemire, J. M. & Levin, M. Bioelectric signaling regulates head and organ size during planarian regeneration. Development 140, 313–322 (2013).
Pai, V. P., Aw, S., Shomrat, T., Lemire, J. M. & Levin, M. Transmembrane voltage potential controls embryonic eye patterning in Xenopus laevis. Development 139, 313–323 (2012).
Pai, V. P. et al. Endogenous gradients of resting potential instructively pattern embryonic neural tissue via notch signaling and regulation of proliferation. J. Neurosci. 35, 4366–4385 (2015).
Slotkin, T. A. If nicotine is a developmental neurotoxicant in animal studies, dare we recommend nicotine replacement therapy in pregnant women and adolescents? Neurotoxicol. Teratol. 30, 1–19 (2008).
Huizink, A. C. & Mulder, E. J. Maternal smoking, drinking or cannabis use during pregnancy and neurobehavioral and cognitive functioning in human offspring. Neurosci. Biobehav. Rev. 30, 24–41 (2006).
Slotkin, T. A. et al. Effects of prenatal nicotine exposure on primate brain development and attempted amelioration with supplemental choline or vitamin C: neurotransmitter receptors, cell signaling and cell development biomarkers in fetal brain regions of rhesus monkeys. Neuropsychopharmacology 30, 129–144 (2005).
Velazquez-Ulloa, N. A. A Drosophila model for developmental nicotine exposure. PLoS ONE 12, e0177710 (2017).
Biel, M., Wahl-Schott, C., Michalakis, S. & Zong, X. Hyperpolarization-activated cation channels: from genes to function. Physiol. Rev. 89, 847–885 (2009).
Qu, Y., Whitaker, G. M., Hove-Madsen, L., Tibbits, G. F. & Accili, E. A. Hyperpolarization-activated cyclic nucleotide-modulated ‘HCN’ channels confer regular and faster rhythmicity to beating mouse embryonic stem cells. J. Physiol. 586, 701–716 (2008).
Spater, D. et al. A HCN4 + cardiomyogenic progenitor derived from the first heart field and human pluripotent stem cells. Nat. Cell Biol. 15, 1098–1106 (2013).
Yasui, K. et al. I f current and spontaneous activity in mouse embryonic ventricular myocytes. Circ. Res. 88, 536–542 (2001).
Vicente-Steijn, R. et al. Funny current channel HCN4 delineates the developing cardiac conduction system in chicken heart. Heart Rhythm 8, 1254–1263 (2011).
Zuber, M. E. Eye field specification in Xenopus laevis. Curr. Top. Dev. Biol. 93, 29–60 (2010).
Fuhrmann, S. Eye morphogenesis and patterning of the optic vesicle. Curr. Top. Dev. Biol. 93, 61–84 (2010).
Burger, C. & Ribera, A. B. Xenopus spinal neurons express Kv2 potassium channel transcripts during embryonic development. J. Neurosci. 16, 1412–1421 (1996).
Pietak, A. & Levin, M. Exploring instructive physiological signaling with the bioelectric tissue simulation engine. Front Bioeng. Biotechnol. 4, 55 (2016).
Harris, A. L., Spray, D. C. & Bennett, M. V. Control of intercellular communication by voltage dependence of gap junctional conductance. J. Neurosci. 3, 79–100 (1983).
Charbonnier, F. et al. Specific activation of the acetylcholine receptor subunit genes by MyoD family proteins. J. Biol. Chem. 278, 33169–33174 (2003).
Papke, R. L., Dwoskin, L. P. & Crooks, P. A. The pharmacological activity of nicotine and nornicotine on nAChRs subtypes: relevance to nicotine dependence and drug discovery. J. Neurochem. 101, 160–167 (2007).
Wang, H., Yang, B., Zhang, L., Xu, D. & Wang, Z. Direct block of inward rectifier potassium channels by nicotine. Toxicol. Appl. Pharmacol. 164, 97–101 (2000).
Kodirov, S. A., Wehrmeister, M. & Colom, L. V. Modulation of HCN channels in lateral septum by nicotine. Neuropharmacology 81, 274–282 (2014).
Adams, D. S. & Levin, M. Measuring resting membrane potential using the fluorescent voltage reporters DiBAC4(3) and CC2-DMPE. Cold Spring Harb. Protoc. 2012, 459–464 (2012).
Pai, V. P., Lemire, J. M., Chen, Y., Lin, G. & Levin, M. Local and long-range endogenous resting potential gradients antagonistically regulate apoptosis and proliferation in the embryonic CNS. Int. J. Dev. Biol. 59, 327–340 (2015).
Xu, X., Vysotskaya, Z. V., Liu, Q. & Zhou, L. Structural basis for the cAMP-dependent gating in the human HCN4 channel. J. Biol. Chem. 285, 37082–37091 (2010).
Moosmang, S. et al. Cellular expression and functional characterization of four hyperpolarization-activated pacemaker channels in cardiac and neuronal tissues. Eur. J. Biochem. 268, 1646–1652 (2001).
Xue, T., Marban, E. & Li, R. A. Dominant-negative suppression of HCN1- and HCN2-encoded pacemaker currents by an engineered HCN1 construct: insights into structure-function relationships and multimerization. Circ. Res. 90, 1267–1273 (2002).
Werner, S., Rink, J. C., Riedel-Kruse, I. H. & Friedrich, B. M. Shape mode analysis exposes movement patterns in biology: flagella and flatworms as case studies. PLoS. One. 9, e113083 (2014).
Webster, M., . & Sheets, H.D. A practical introduction to landmark-based geometric morphometrics. Quant. Methods Paleobiol. 16, 163–188 (2010).
Blackiston, D., Shomrat, T., Nicolas, C. L., Granata, C. & Levin, M. A second-generation device for automated training and quantitative behavior analyses of molecularly-tractable model organisms. PLoS ONE 5, e14370 (2010).
Rothman, G. R., Blackiston, D. J. & Levin, M. Color and intensity discrimination in Xenopus laevis tadpoles. Anim. Cogn. 19, 911–919 (2016).
Blackiston, D. J. & Levin, M. Aversive training methods in Xenopus laevis: general principles. Cold Spring Harb Protoc. https://doi.org/10.1101/pdb.top068338 (2012).
Blackiston, D. J. & Levin, M. Ectopic eyes outside the head in Xenopus tadpoles provide sensory data for light-mediated learning. J. Exp. Biol. 216, 1031–1040 (2013).
Blackiston, D., Khanh, V. & Levin, M. Serotonergic stimulation induces nerve growth and promotes visual learning via posterior eye grafts in a vertebrate model of induced sensory plasticity. NPJ Regen. Med. 2 10.1038/s41536-017-0012-5 (2017).
Acampora, D. et al. Forebrain and midbrain regions are deleted in Otx2-/- mutants due to a defective anterior neuroectoderm specification during gastrulation. Development 121, 3279–3290 (1995).
Bourguignon, C., Li, J. & Papalopulu, N. XBF-1, a winged helix transcription factor with dual activity, has a role in positioning neurogenesis in Xenopus competent ectoderm. Development 125, 4889–4900 (1998).
Georgala, P. A., Carr, C. B. & Price, D. J. The role of Pax6 in forebrain development. Dev. Neurobiol. 71, 690–709 (2011).
Muzio, L. & Mallamaci, A. Emx1, emx2 and pax6 in specification, regionalization and arealization of the cerebral cortex. Cereb. Cortex 13, 641–647 (2003).
Adams, D. S. & Levin, M. Endogenous voltage gradients as mediators of cell-cell communication: strategies for investigating bioelectrical signals during pattern formation. Cell. Tissue Res. 352, 95–122 (2013).
Wolpert, L. Positional information and pattern formation. Curr. Top. Dev. Biol. 117, 597–608 (2016).
Tsikolia, N. The role and limits of a gradient based explanation of morphogenesis: a theoretical consideration. Int. J. Dev. Biol. 50, 333–340 (2006).
Briscoe, J. & Small, S. Morphogen rules: design principles of gradient-mediated embryo patterning. Development 142, 3996–4009 (2015).
Hernandez-Diaz, S. & Levin, M. Alteration of bioelectrically-controlled processes in the embryo: a teratogenic mechanism for anticonvulsants. Reprod. Toxicol. 47, 111–114 (2014).
Masotti, A. et al. Keppen-Lubinsky syndrome is caused by mutations in the inwardly rectifying K + channel encoded by KCNJ6. Am. J. Hum. Genet. 96, 295–300 (2015).
Kortum, F. et al. Mutations in KCNH1 and ATP6V1B2 cause Zimmermann-Laband syndrome. Nat. Genet. 47, 661–667 (2015).
Veale, E. L., Hassan, M., Walsh, Y., Al-Moubarak, E. & Mathie, A. Recovery of current through mutated TASK3 potassium channels underlying Birk Barel syndrome. Mol. Pharmacol. 85, 397–407 (2014).
Sive, H., Grainger, R. M. and Harland, R. Early development of Xenopus laevis.(Cold Spring Harbor Laboratory Press, New York, 2000).
Nieuwkoop, P.D. & Faber, J. Normal table of Xenopus laevis (Daudin), Ed 2. Amsterdam: North-Holland Publishing Company (1967).
Schneider, C. A., Rasband, W. S. & Eliceiri, K. W. NIH Image to ImageJ: 25 years of image analysis. Nat. Methods 9, 671–675 (2012).
Klingenberg, C. P. MorphoJ: an integrated software package for geometric morphometrics. Mol. Ecol. Resour. 11, 353–357 (2011).
Rohlich, P. & Szel, A. Photoreceptor cells in the Xenopus retina. Microsc. Res. Tech. 50, 327–337 (2000).
Pannese, M. et al. The Xenopus homologue of Otx2 is a maternal homeobox gene that demarcates and specifies anterior body regions. Development 121, 707–720 (1995).
Eagleson, G. W., Johnson-Meeter, L. J. & Frideres, J. Effects of retinoic acid upon eye field morphogenesis and differentiation. Dev. Dyn. 221, 350–364 (2001).
Eagleson, G. W. & Theisen, S. Stage-specific effects of retinoic acid on gene expression during forebrain development. Brain. Res. Bull. 75, 281–288 (2008).
Herrera-Rincon, C., Pai, V. P., Moran, K. M., Lemire, J. M. & Levin, M. The brain is required for normal muscle and nerve patterning during early Xenopus development. Nature. Communications 8, 587 (2017).
We thank Erin Switzer and Rakela Colon for Xenopus husbandry and general lab assistance, Dany Adams for help with microscopy, Valerie Schneider for otx2 anti-sense probe, Gerald Eagleson for emx and xbf1 anti-sense probe, David Paul for H7 construct, and Randy Blakely for DN-SERT construct. We thank Jean-Francois Pare and Joan Lemire for assistance with cloning of cDNAs into injection vectors PCS2. We thank Douglas Blackiston for assistance with learning behavior assays. We thank Kelly McLaughlin, Emily Pitcairn, and Joshua Finkelstein for their helpful suggestions and comments on the manuscript. We gratefully acknowledge support of the Allen Discovery Center program through The Paul G. Allen Frontiers Group (12171). We also gratefully acknowledge support from the W.M. Keck Foundation (5903), the G. Harold and Leila Y. Mathers Charitable Foundation (TFU141), the Templeton World Charity Foundation (TWCF0089/AB55), National Institutes of Health (AR055993-01, AR061988), and The American Heart Association National Center (0435030 N, 0630268 N).
The authors declare no competing interests.
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Pai, V.P., Pietak, A., Willocq, V. et al. HCN2 Rescues brain defects by enforcing endogenous voltage pre-patterns. Nat Commun 9, 998 (2018). https://doi.org/10.1038/s41467-018-03334-5
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