TrkB dependent adult hippocampal progenitor differentiation mediates sustained ketamine antidepressant response

Ma, Zhenzhong; Zang, Tong; Birnbaum, Shari G.; Wang, Zilai; Johnson, Jane E.; Zhang, Chun-Li; Parada, Luis F.

doi:10.1038/s41467-017-01709-8

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Published: 21 November 2017

TrkB dependent adult hippocampal progenitor differentiation mediates sustained ketamine antidepressant response

Zhenzhong Ma ORCID: orcid.org/0000-0002-1235-3765^1,2,
Tong Zang³,
Shari G. Birnbaum⁴,
Zilai Wang¹^nAff5,
Jane E. Johnson²,
Chun-Li Zhang ORCID: orcid.org/0000-0002-2639-4605³ &
…
Luis F. Parada¹^nAff5

Nature Communications volume 8, Article number: 1668 (2017) Cite this article

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Abstract

Adult neurogenesis persists in the rodent dentate gyrus and is stimulated by chronic treatment with conventional antidepressants through BDNF/TrkB signaling. Ketamine in low doses produces both rapid and sustained antidepressant effects in patients. Previous studies have shed light on post-transcriptional synaptic NMDAR mediated mechanisms underlying the acute effect, but how ketamine acts at the cellular level to sustain this anti-depressive function for prolonged periods remains unclear. Here we report that ketamine accelerates differentiation of doublecortin-positive adult hippocampal neural progenitors into functionally mature neurons. This process requires TrkB-dependent ERK pathway activation. Genetic ablation of TrkB in neural stem/progenitor cells, or pharmacologic disruption of ERK signaling, or inhibition of adult neurogenesis, each blocks the ketamine-induced behavioral responses. Conversely, enhanced ERK activity via Nf1 gene deletion extends the response and rescues both neurogenic and behavioral deficits in mice lacking TrkB. Thus, TrkB-dependent neuronal differentiation is involved in the sustained antidepressant effects of ketamine.

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Introduction

Major depressive disorder (MDD) is a significant cause of disability worldwide, having a devastating impact on both individuals and society¹. Currently, available antidepressant drugs typically modulate monoaminergic neurotransmission and take several weeks to months to exert their biological effects and achieve clinical efficacy². Moreover, over half of patients with major depression do not have an appreciable response to conventional monoamine re-uptake inhibitor-based therapy^3,4. In clinical studies, a single low dose of ketamine, a non-competitive glutamatergic N-methyl-D-aspartate receptor (NMDAR) antagonist, produced both fast-acting and sustained antidepressant effects in patients resistant to conventional antidepressants and at high suicide risk^5,6,7. Several mechanisms have been proposed for these acute ketamine antidepressant effects that can be observed within 1 h of administration in rodents. Among the invoked underlying mechanisms are suppression of spontaneous neurotransmission mediated NMDAR activation with subsequent enhanced BDNF protein synthesis in the hippocampus^8,9, and rapid synaptic dysfunction recovery through mTOR pathway activation in the prefrontal cortex^10,11. However, the mechanisms underlying the more extended action of ketamine are not fully understood and remain the subject of intense investigation.

For over a decade, the role of neurotrophic factors in the etiology of depression and the anti-depressive response has been well documented¹². In rodent models, brain-derived neurotrophic factor (BDNF) and the signaling by its receptor tyrosine kinase, TrkB, have been implicated in stress and mounting the anti-depressive response of selective monoamine reuptake inhibitors. Chronic stress decreases BDNF levels in the hippocampus and causes neuronal atrophy and cell death. In adult nonhuman primates, hippocampal neurogenesis is impaired by stress and can be stimulated by stress coping causing improvement in antidepressant activity^13,14. Conversely, chronic antidepressant treatment elevates BDNF expression, supports neuronal survival, and enhances proliferation of neural progenitor cells (NPCs) in the subgranular zone (SGZ) of the dentate gyrus (DG). Enhanced NPC proliferation eventually drives increased neurogenesis and the enhanced behavioral response to antidepressant exposure^12,15,16. Additional observations implicating hippocampal neurogenesis in mood control include that irradiation-mediated or genetic suppression of adult hippocampal neurogenesis compromises the chronic antidepressant effect and stress responses^17,18. An increase in new cell generation has also been reported in human depression patients who received antidepressant treatment before death¹⁹. Our own previous studies have demonstrated that in mouse models, BDNF/TrkB signaling in hippocampal neural progenitor cells (NPCs) regulates behavioral sensitivity to conventional antidepressants^20,21.

Ketamine antidepressant effect does not involve serotonin reuptake inhibition. It is known to stimulate rapid BDNF expression in the hippocampus through a translation mechanism by which phosphorylated eukaryotic elongation factor 2 (eEF2) becomes reduced in both neuronal somata and dendrites⁸. Given that specific subtypes of Bdnf mRNA transcripts are locally translated for secretion in an activity-dependent manner in somata²², ketamine treatment could render BDNF protein accessible to the neurogenic niche of the DG. This raises interesting questions regarding how the rapid biological effects of NMDAR blockade might relate to the more latent actions of monoamine reuptake inhibition, and whether BDNF/TrkB mediated hippocampal neurogenesis may represent a nexus for both mechanisms.

In the present study, we examine the effects of ketamine on hippocampal neurogenesis and find that ketamine accelerates doublecortin (DCX) positive progenitor differentiation into mature neurons within 24 h. Genetic or pharmacologic disruption of DCX+ progenitor differentiation results in a blockade of the sustained behavioral response induced by ketamine. We further identify TrkB signaling and its downstream ERK pathway activation as essential for the generation of newborn neurons and consequent behavioral responses. Moreover, the enhancement of ERK activity by genetically deleting Nf1 in adult DG progenitors, not only prolongs the ketamine antidepressant response but also rescues both the neurogenic and behavioral deficits in TrkB mutant mice. Our results establish an essential role for BDNF/TrkB-dependent adult hippocampal neurogenesis in maintaining ketamine-mediated antidepressant effects and provide support for the notion that hippocampal neurogenesis is an essential modulator of depression.

Results

Ketamine accelerates DG progenitor cell differentiation

To investigate a potential role for adult hippocampal neurogenesis in mediating ketamine antidepressant effects, we first examined adult hippocampal neurogenesis following administration of the same dose (7 mg/kg) that is sufficient to induce behavioral response⁸. Twenty-four hours after treatment, mice had normal neural progenitor cell (NPC) proliferation and differentiation as measured by Ki67+ and DCX+ cell number respectively (Supplementary Fig. 1a). Analysis at 1 week showed an increased DCX+ progenitor cell number (Supplementary Fig. 1b). In the adult hippocampus, radial glia-like neural stem/progenitor cells (Nestin+) give rise to DCX+ progenitors over a two week period that progress into mature neurons (NeuN+, DCX−) in the third week (Fig. 1a). A BrdU pulse-chase experiment to label proliferating NPCs (Supplementary Fig. 1c) revealed that the ketamine increased BrdU incorporation was not present in the DCX positive newborn cells (DCX+/BrdU+) 1 week after treatment (Supplementary Fig. 1d, e). Instead as shown below, the BrdU was prematurely chased into the newborn neuron (NeuN) population. We saw no evidence of enhanced NPC proliferation or DCX+ progenitor cell number indicating that early phases of neurogenesis were unaffected. To better examine the late phase of neurogenesis, we next performed a BrdU pulse to label the proliferating neural progenitors and chased them for either 19 or 25 days with ketamine exposure at day 18 (Fig. 1b). The data show that one dose of ketamine accelerated newborn neuron (NeuN+, DCX−) generation among the BrdU+ cells at both 24 h (day 19) and 1-week (day 25) post-treatment (Figs 1c, d). Correspondingly, the increase in newborn neurons was accompanied by a decrease in DCX+ cells among BrdU+ cells at both time points (Fig. 1e). Accelerated differentiation of DCX+ progenitors to NeuN+ mature neurons was also observed when we traced the nestin+ neural stem/progenitor cell lineage in the DG with a Rosa26-tdTOM reporter (Supplementary Fig. 1f–i), driven by a tamoxifen-inducible Nestin-creER^T2 transgene that is highly efficient and specific in targeting the vast majority of neural stem/progenitor cells in the DG^21,23 (Supplementary Fig. 2a). Taken together, these data indicate that ketamine exerts no effects on quiescent stem cell activation, or transition to DCX+ cells, but instead promotes accelerated differentiation of existing DCX+ progenitors into newborn neurons.

Newborn neurons are functionally mature

To examine whether newborn neurons resulting from ketamine treatment are functional and integrate into the existing DG neural circuitry, we studied their electrophysiological properties by taking whole-cell patch clamp recordings. Recorded neurons were traced by using Nestin-CreER^T2 –tdTomato to ensure they originated from NPCs in the DG (Fig. 2a). By morphology, newborn neurons following ketamine treatment display normal dendritic branching, including secondary/tertiary dendrites and dendritic tips, compared with controls (Fig. 2b). All recorded newborn neurons fired repetitive action potentials (APs) upon current injection when examined at 24 h after saline or ketamine treatment (Fig. 2c), and had inward and outward currents in voltage-clamp mode, through voltage-gated sodium and potassium channels, respectively (Supplemental Fig. 2e). The neurons from saline and ketamine treatment showed similar intrinsic cell properties, including capacitance, input resistance, and resting membrane potential (Figs 2d–f). They also showed similar excitability, including AP after hyperpolarization, half width, threshold, amplitude, frequency (Figs. 2g–k) and delay of the first spike, the maximum velocity of rising and decay (Supplemental Fig. 2b–d). There were no significant differences in channel properties among these differentiated neurons, as measured by sodium and potassium current amplitudes (Supplemental Fig. 2f–h). Importantly, typical spontaneous postsynaptic currents (sPSCs) were detected, indicating functional synapse formation between these neuron populations and local neural circuitry (Fig. 2l). Saline or ketamine treatment had similar frequency and amplitude of sPSCs, suggesting the comparable synapse connectivity when ketamine-induced newborn neurons integrated into the local network (Figs. 2m, n). Thus, morphological and electrophysiological analysis of ketamine exposed newborn hippocampal neurons indicated normal differentiation and activity.

We further assessed the response of ketamine exposed newborn neurons to pathological states by the induction of seizures. The chemoconvulsant, kainic acid (KA), is a potent agonist of glutamate kainate receptors and systemic administration induces seizures with classic immediate early gene transcription response in the hippocampus^24,25. Thus, newborn neurons that incorporate into the hippocampal circuitry will respond to the KA stimulated neuro-excitation wave and exhibit an immediate early gene response including the well-characterized immediate early response gene, EGR1 that is a marker of the maturity of adult-born hippocampal granule neurons^26,27. Mice were subjected to BrdU pulses and chased for 18 days to allow time for BrdU presence in late stage progenitors and newborn neurons. Two hours after KA was administered, mice were killed and assayed for co-expression of BrdU and EGR1 (Supplementary Fig. 3a). KA induction leads to EGR1 activation in hippocampal neurons in all animals, exhibiting a similar percentage of triple positive cells (>80%; BrdU+/NeuN+/EGR1+) in newborn neurons (BrdU+/NeuN+) (Supplementary Fig. 3d, e, f). However, consistent with the finding that ketamine accelerates newborn neuron generation (Fig. 1), ketamine-treated animals exhibited an increased number of EGR1 expressing newborn neurons (BrdU+/NeuN+/EGR1+) (Supplementary Fig. 3b, c). Thus, by the above criteria, newborn neurons arising from ketamine accelerated progenitor differentiation are functionally mature and exhibit similar synaptic activation as normal newborn neurons in both physiologic and pathologic states.

DCX+ progenitor differentiation sustains ketamine effect

To further explore the physiologic relevance of accelerated DCX+ to NeuN+ cell differentiation in the behavioral response to ketamine, we selectively eliminated Nestin+ neural stem cells and their immediate progeny prior to ketamine exposure using a floxed-STOP-diphtheria toxin subunit A (DTA) transgene embedded within the Rosa26 locus that was activated by Nestin-creER^T2 transgene (DTA^Nes)²⁸. Adult DTA^Nes mice were treated with tamoxifen to activate DTA expression followed by saline or ketamine treatment eighteen days later (Fig. 3a). This eighteen-day induction paradigm restricts DTA elimination to stem cells and progenitors that would have normally been produced within the eighteen-day period but minimally affects newborn or mature neurons that were formed prior to the induction. Nestin-creER^T2 induced recombination is restricted to the neurogenic niches (SGZ and SVZ) in adult brain (Supplementary Fig. 4), and thus DTA^Nes tamoxifen-treated mice did not display cell loss in other brain regions and were indistinguishable from their littermate controls in brain morphology, brain weight and structures (Supplementary Fig. 5). However, adult neurogenesis was efficiently eliminated, with complete loss of Ki67 positive proliferating NPCs and dramatic reduction of DCX+ cell number (5% remaining compared to control) in the DG (Fig. 3b). Pre-existing mature neurons and astrocytes appeared to be unaffected in DTA^Nes mice (Supplementary Fig. 5d–g). Moreover, DTA^Nes neurogenesis-deficient mice were rendered insensitive to the anti-depressive effects of ketamine 24 h after treatment as observed in both the forced swim test (FST) and novelty-suppressed feeding test (NSFT) (Figs. 3c, d). These data indicate that the late-stage progenitor (DCX+) pool normally available for conversion into mature neurons, but eliminated in this paradigm by DTA, is essential for the sustained behavioral response to ketamine.

We also used a pharmacologic approach to target proliferating neural progenitor cells in the hippocampus. Temozolomide (TMZ) is a DNA alkylating agent in use to treat patients suffering from glioblastoma multiforme where it targets the BrdU-incorporating (dividing) tumor cell population and transiently arrests tumor growth²⁹. This potent chemotherapeutic agent has also been shown to effectively impair adult hippocampal neurogenesis in mouse models of learning and memory³⁰. As shown in Supplementary Fig. 6, TMZ impairs adult hippocampal neurogenesis, as measured by both Ki67 and DCX. To avoid any potential confounding side effects of acute TMZ treatment on behavior assays, mice were subjected to four TMZ cycles followed by a 1-month gap prior to behavioral testing (Fig. 4a). This paradigm results in the selective reduction of late-phase DCX+ progenitors. After termination of TMZ treatment, recovery of the progenitor population is mediated by quiescent cell re-entry into the cell cycle. Indeed, the TMZ-treated mice have the same number of total DCX+ cells as controls, but are overrepresented by early progenitors (DCX+/Ki67+) compared to controls (Figs. 4b, d, e). Consistent with the experimental design, the DCX+ progenitor population following TMZ treatment exhibits properties of newly formed immature progenitors including reduced dendritic processing and proximity to their source in the subgranular zone (SGZ). In contrast, vehicle treated mice have abundant numbers of late phase progenitors (56.0% ± 2.41 vs 23.2% ± 3.05) with established dendritic morphology extending through the granular layer zone (GLZ) into the molecular layer (Figs. 4b, c and f). These data are consistent with the model that TMZ treatment results in a greatly reduced source of the late-phase progenitors for the production of newborn neurons. Upon treatment arrest, quiescent stem cells re-enter the cell cycle aggressively to compensate for the early progenitor loss caused by the drug exposure. As shown in Fig. 4g, although both vehicle and TMZ-treated mice respond to ketamine by accelerating newborn neuron production, TMZ mice have a markedly impaired capacity and only exhibit about 20% of new neurons generated in ketamine-treated vehicle mice. Consistent with the previous DTA experiment, the consequence of TMZ treatment and progenitor cell destruction is a blockade of the ketamine anti-depressive behavior effect in FST (Fig. 4h). Taken together, the genetic lineage ablation and pharmacological studies indicate that ketamine exerts its sustained anti-depressive behavior by accelerating the formation of newborn neurons from the pre-existing pool of mature DCX+ progenitors.

TrkB mediates ketamine antidepressant effect

In the hippocampus, ketamine accelerates DCX+ progenitor differentiation within 24 h (Fig. 1), which correlates with the rapid and significant increase in BDNF protein levels observed in the DG (Fig. 5a). Previous studies have shown that BDNF plays an important role in NPC survival, proliferation, differentiation and the behavioral response to chronic treatment with conventional antidepressants^20,21,31,32. TrkB, the primary receptor for BDNF, is expressed in the entire neural progenitor lineage in adult mouse DG^20,33. Therefore we tested a possible role for TrkB in the ketamine-induced acceleration of DCX+ progenitor differentiation and the anti-depressive behavioral response. Using Nestin-creER^T2 mice, we specifically ablated TrkB (TrkB flox/flox) in the adult neural progenitor lineage (TrkB^Nes) and exposed the TrkB deficient mice to different anti-depressive behavioral tests six weeks after tamoxifen induction (Supplementary Fig. 7a). Although TrkB ablation in the adult DG did not alter the basal level of depression-like behavior in mice²⁰, the ketamine antidepressant behavioral effect was fully blocked as measured by immobility in the FST and feeding latency in the NSFT (Supplementary Fig. 7b, c). By the end of the NSFT (10 min), 81.8% of ketamine-treated control mice had fed compared with 66.7% of TrkB^Nes f/f mice (Supplementary Fig. 7d). All mice consumed similar food quantity following the latency test, indicating that the behavioral change was not caused by altered appetite or motivation to feed (Supplementary Fig. 7e). In the learned helplessness test, the ketamine-treated TrkB^Nes mice escaped in fewer trials compared with ketamine-treated control animals (7.85 ± 1.22 vs 11.46 ± 0.89) (Supplementary Fig. 7f). Also, unlike control animals that responded to ketamine and displayed significantly shorter escape latencies, TrkB^Nes mice had an attenuated ketamine response at the beginning of the test (trials 4–9 of total 15 trials) but did eventually learned to escape from the chamber (Supplementary Fig. 7g). The data indicate that TrkB is critical in adult newborn neurons for mounting ketamine anti-depressive behavioral response.

To further investigate the role of TrkB in mediating DCX+ progenitor differentiation and ketamine action, we employed a 3-week post tamoxifen induction paradigm to target TrkB ablation to NPCs while minimizing TrkB loss in newborn mature granule neurons (Fig. 5b). As anticipated, control mice exhibit accelerated neuronal differentiation 24 h after ketamine treatment. In contrast, mice with TrkB deleted NPCs had impaired generation of newborn neurons and instead an increased percentage of DCX+ progenitors compared with ketamine-treated control mice (Figs 5c, d). Therefore, ketamine mediates increased total number of newborn neurons in the DG that can be blocked by TrkB ablation (Supplementary Fig. 7h). Accordingly, TrkB mutant mice displayed significantly increased immobility time in the FST compared with control mice at both 24 h and 1 week after ketamine treatment (Figs. 5f, g). Similar results were seen in the NSFT where feeding latency was not affected by ketamine treatment in TrkB^Nes mice (Fig. 5h). Moreover, cumulative feeding latency analysis revealed that when 100% of ketamine-treated control mice had fed, only 31% of ketamine-treated TrkB^Nes mice had fed (Fig. 5I). This difference cannot be attributed to altered appetite because all groups of mice consumed food equally with equivalent feeding behavior (Fig. 5J). Importantly, by virtue of the 3-week tamoxifen paradigm, these TrkB mutant mice retained the acute (1 h) anti-depressive response to ketamine (Fig. 5e), which is mediated by fast-acting synaptic mechanisms in pre-existing mature neurons that are not affected by this paradigm^8,10. Thus sustained ketamine behavioral response as well as the accelerated progenitor differentiation requires functional TrkB.

TrkB-dependent signal transduction regulates ketamine effect

To elucidate the mechanism by which hippocampal progenitor differentiation is accelerated by ketamine-induced BDNF/TrkB signaling, we examined the major effector pathways, that have been implicated in BDNF/TrkB signaling^21,22,34,35. Given that ketamine has a short half-life (~3 h)⁸ and can increase BDNF protein levels within 1 h (Fig. 5a), we examined early responses of signaling pathways by measuring phosphorylation levels of TrkB, ERK (RAS/MAPK pathway), AKT (PI3K pathway) and S6 (mTOR pathway) in the DG. We observed enhanced ERK phosphorylation, but not AKT or S6 after ketamine treatment (Fig. 6a). Importantly, in TrkB^Nes DCX+ progenitors, p-ERK was equivalent to controls (Supplementary Fig. 9a), consistent with a requirement for BDNF/TrkB signaling to induce ERK activation. We further observed that immature DCX+ progenitors had relatively higher ERK phosphorylation than more mature progenitors (Fig. 6b), indicating that DCX+ progenitors have differential ERK activation response to ketamine. Ketamine also induced ERK mild activation in the CA1, but not in the CA3 and cerebellum (Supplementary Fig. 9b). Western blot analysis from isolated DG tissue confirmed that ketamine-induced a TrkB-dependent activation of the ERK pathway (Figs 6c, d). Interestingly, ERK activation seems to be transient in mature hippocampal neurons. ERK phosphorylation disappeared in the granular layer but was maintained in neural progenitors 24 h after ketamine treatment (Supplementary Fig. 9c).

To directly test the role of ERK pathway activation in mediating hippocampal progenitor differentiation and the behavioral response to ketamine, we pretreated mice with a selective MEK inhibitor, SL327³⁶, 1 h before ketamine treatment (Fig. 7a). This pre-treatment suppressed ketamine-mediated ERK activation by 25% as measured by normalized ERK phosphorylation from dissected DG (Supplementary Fig. 8a, b). One day after ketamine treatment, we subjected mice to FST. One dose of SL327, 24 h prior to behavioral testing did not alter the depression-like behavior in saline-treated mice⁸; However, SL327 pretreatment blocked the ketamine antidepressant effect (Fig. 7c), similar to that observed in TrkB mutant mice. Moreover, the generation of newborn DG neurons was also impaired as demonstrated by the reduction of BrdU+ cells expressing NeuN in the SL327 treated cohort (Fig. 7b). These data are consistent with our model that TrkB-dependent ERK activation is required for ketamine-induced progenitor differentiation and antidepressant response.

A prediction from the preceding studies would be that enhanced or prolonged ERK activation in DG NPCs should promote both the neurogenic and behavioral responses to ketamine. To enhance ERK activation specifically in adult NPCs, we turned to a genetic approach. The protein encoded by the NF1 tumor suppressor, neurofibromin, is a demonstrated negative regulator (RAS-GAP) downstream of the Trk family of receptor tyrosine kinases^21,34,37. We used Nes-creER^T2 to genetically delete Nf1 in adult hippocampal stem cells and their progeny (NF1^Nes). Adult NF1^Nes mice were treated with tamoxifen to delete Nf1 three weeks prior to saline or ketamine administration (Fig. 7d). Twenty-four hours later, the analysis of neurogenesis revealed that NF1^Nes mice exhibited enhanced generation of hippocampal newborn neurons comparable to the ketamine effect on control mice (Fig. 7e). We also observed that in the absence of NF1, ketamine had no additional effect on newborn neuron production indicating a saturation of neuronal differentiation. Similar to what we have previously reported, DCX+ progenitors with NF1 loss mediated enhanced p-ERK level (Supplementary Fig. 8c), continuously produce adult-born neurons in mutant mice²¹. Behavioral tests four weeks after ketamine treatment indicated that both NF1^Nes heterozygous and homozygous mice, but not control mice, maintained the antidepressant effect of ketamine (Fig. 7f). Thus pharmacologic or genetic manipulation to activate the ERK signal transduction pathway in NPCs improves the behavioral anti-depressive response to ketamine.

Enhanced ERK pathway rescues phenotype in TrkB mutants

To close the circle, given the inhibition of cellular and physiological response to ketamine after genetic TrkB loss and the acceleration following ERK activation, we directly examined epistasis between NF1 and TrkB. Nestin-creER^T2 was combined with both the TrkB and NF1 floxed alleles (TrkB^Nes; NF1^Nes). In the same paradigm used for TrkB mutants (Fig. 5b), three weeks after dual TrkB and NF1 ablation in hippocampal progenitors, mice were subjected to the FST behavioral assay. Consistent with previous results, ketamine induced a decreased immobility time in control, double heterozygote mutant, and NF1 mutant mice, but not in TrkB mutant mice. In contrast, the inclusion of one floxed allele of Nf1 (TrkB^Nes; NF1^Nes) was sufficient to rescue the impaired behavioral response to ketamine (Fig. 8a). Moreover, at the cellular level, Nf1 ablation successfully reversed the low p-ERK expression in DCX+ cells observed in TrkB^Nes mice following ketamine treatment (Supplementary Fig. 9a). Commensurately, the deficiency of accelerated neuronal differentiation present in TrkB^Nes mice was also rescued by co-introduction of an NF1 knock-out allele. A significantly higher percentage of newborn neurons was present in TrkB^Nes; NF1^Nes double-mutant mice compared with ketamine-treated TrkB^Nes mice (Fig. 8b). Consequently, the abolished enhancement of newborn neuron generation by TrkB ablation could be maintained in the ketamine-treated TrkB^Nes; NF1^Nes double-mutant mice (Fig. 8c). These results demonstrate a linear signaling relationship between TrkB and ERK pathway function in mediating both hippocampal progenitor differentiation and mounting a behavioral effect in response to acute ketamine induction.

Discussion

The continuous generation of new neurons by NPCs in the dentate gyrus provides structural plasticity in the adult dentate gyrus allowing for behavioral response to environmental stimuli, including antidepressants. It has been demonstrated that the almost immediate acute, behavioral response to ketamine can be explained by rapid synaptic plasticity changes and circuit rewiring⁹. Our study provides a functional link between adult hippocampal neurogenesis and the more sustained anti-depressive response to ketamine in mice. By extension and analogy, it provides support for the notion that adult hippocampal neurogenesis is a critical biological determinant of the anti-depressive response¹². Consistent with previous studies showing that in the hippocampus, BDNF plays a central role in neuronal differentiation and maturation^20,22,24, this work demonstrates that ketamine-mediated production of BDNF accelerates DCX+ progenitor differentiation into mature granule neurons through TrkB signaling and downstream ERK pathway activation. This cellular effect elicits a behavioral anti-depressive response within 24 h and the production of newborn progenitors and neurons seems to last for about 1 week. Specific loss of neural progenitor cells in the DTA^Nes and TMZ paradigms significantly impaired the sustained ketamine behavioral response, but not the depression-like behaviors at the baseline that requires newborn mature neurons¹⁸. We also demonstrate that ketamine acceleration of DCX+ progenitors results in functional newborn neurons that likely serves to modulate the hippocampal neural network to sustain the anti-depressive effect analogous to that observed for chronic monoamine treatment¹².

A recent related study in rats reported that ketamine can promote rapid maturation of hippocampal newborn neurons as defined by the immediate early EGR1 (zif268) gene response, leading to the generation of more neurons within hours in both normal conditions and in a depression model²⁵. This study also reported that the acute anti-depressive effect (1 h) is independent of newborn neurons, which is consistent with our finding that enhanced neurogenesis is required for the sustained antidepressant response to ketamine, but not the fast-acting behavioral effect that remains intact in TrkB^Nes mice with neurogenesis deficiency (Fig. 5c & Supplementary Fig. 7h). Whether adult neurogenesis sustains ketamine action in the stressed animal was not directly tested. However, given that ketamine and adult-born neurons behaviorally regulate the stress response^8,13,18,38, it is likely that adult neurogenesis is also required for ketamine-induced recovery of a depression-like state. Thus, ketamine-induced BDNF/TrkB signaling, not only modulates synaptic circuitry in the hippocampus, but also regulates adult hippocampal neurogenesis, both of which may work together to sustain ketamine’s anti-depressive response.

The survival of DCX+ neural progenitors in the SGZ is regulated by neurotransmitters and neurotrophins^22,39. Chronic treatment with conventional antidepressants promotes neural progenitor cell survival through enhanced BDNF signaling. Interestingly, our results showing that a low dose of ketamine mediates accumulation of newborn DCX+ progenitors not accounted for by progenitor proliferation and production suggests a survival effect on NPCs (Supplementary Fig. 1). However, this cellular effect that leads to the generation of new neurons and rewiring of neuronal circuits might be more likely to contribute to more latent behavioral responses rather than to the rapid action examined here.

The RAS-ERK pathway is critical for neurotrophin-mediated neuronal survival, differentiation, and activity^22,40. In the brain, dysfunction of ERK signaling has been associated with impaired neural development and deficits in learning and memory⁴¹. Here we add to the repertoire of ERK functions as a mediator of hippocampal progenitor cell differentiation. Although mTOR activation in prefrontal cortical neurons has been suggested to underlie the acute (1–2 h) action of ketamine¹¹, it is likely that different cell types or brain regions use selective signal transduction elements in the rapid response to ketamine. In addition, the transient ERK response ( < 24 h) coincides with the ketamine-induced temporal change in BDNF protein level in the DG, suggesting a BDNF dependent ERK signaling cascade. This view is supported by the studies of TrkB ablation that resulted in a block of ERK activation and anti-depressive response to ketamine. We also observed differential ERK activation between immature and mature DCX+ progenitors in response to ketamine, which is consistent with the long-term survival effect on NPCs and also echoes previous findings that more proliferative progenitors have higher TrkB expression compared with mature progenitors that have exited the cell cycle^20,33.

The Nf1 gene encodes a tumor suppressor that through RAS-GAP activity, functions as a negative regulator of the RAS pathway⁴². Although NF1 can regulate both the ERK and AKT pathways, in hippocampal NPCs and their progeny, NF1^Nes mice exclusively display ERK activation^21,43. ERK activation via NF1 ablation in NPCs enabled hippocampal progenitors to accelerate differentiation into mature granule neurons, which not only prolonged the behavioral response to ketamine but also restored both the neurogenic and behavioral impairments observed in the TrkB^Nes mice. The results support previous studies showing that ERK signaling is tightly linked to depression etiology and antidepressant treatment^21,44. However, enhanced neuronal differentiation in itself is not sufficient to achieve acute anti-depressive-like behavior in our model system. The NF1^Nes mice display constitutively enhanced neurogenesis but did not show antidepressant-like behavior until treated with ketamine (Figs. 7e, f). Therefore, this neurogenic response likely contributes to the effect together with other mechanisms that underlie ketamine anti-depressive actions^9,10.

Chronic exposure to conventional antidepressants like SSRIs enhances neurogenesis by promoting stem cell entry into the cell cycle and enhancing NPC proliferation. One attractive explanation for the delay in anti-depressive action of conventional antidepressants is the time required to gradually increase BDNF, which then stimulates neural stem/progenitor cell proliferation and eventual production of functional newborn neurons, ultimately leading to behavioral effects^12,20. Ketamine instead accelerates the process through shortcuts involving rapid BDNF translation to promote the generation of functional newborn neurons within 24 h to sustain the AD response. We speculate that the acute or gradual stimulation of BDNF/TrkB signaling may have distinct effects on the regulation of neural stem/progenitor cell behavior (Supplementary Fig. 10). This idea is partially supported by previous in vitro studies that acute and gradual modulation of BDNF signaling produces opposing effects on hippocampal neuron activity owing to the differential kinetics of TrkB activation and downstream signaling including ERK pathway⁴⁵, suggesting that temporal aspects of BDNF/TrkB signaling may be crucial for regulating neural stem/progenitor cell biology. Understanding of the timing and scope of BDNF action upon induction by antidepressants will still require additional study. It will further be of interest to investigate the neurogenesis related mechanistic underpinnings for the ketamine metabolite, (2 R, 6 R)-hydroxynorketamine (HNK), recently reported to produce both rapid and sustained AD effect in an NMDAR inhibition-independent manner⁴⁶. This effect may also be mediated by BDNF signaling and neural progenitor differentiation/maturation as described here for the sustained ketamine antidepressant effect.

Methods

Mice

TrkB^flox mice³⁴, NF1^flox mouse line⁴², Rosa26-DTA mice (The Jackson lab, stock# 006331)²⁸ and Nestin-creER^T2 transgenic mice^20,23 were generated as described previously. Rosa26-LacZ, YFP, and tdTOM reporter lines are from JAX (#003474, 025109 and 007914, respectively).All animals in these studies were maintained on 129/SvEv and C57BL/6 mixed background. TrkB^Nes or Nf1^Nes mutant mice were generated by interbreeding TrkB flox/flox or NF1 flox/flox mice with TrkB^Nes flox/flox or NF1^Nes flox/flox mice, respectively. TrkB^Nes; NF1^Nes double-mutant mice were generated from the interbreeding between TrkB^Nes flox/+; NF1^Nes flox/+ double heterozygotes mice. Only DTA^Nes heterozygote mice were used in the experiments and generated by breeding DTA^R26 with Nestin-creER^T2. Control animals used in the experiments were either tamoxifen-induced mice that did not have the Nestin-creER^T2 transgene, or oil vehicle treated mice without DTA^R26, TrkB^flox and Nf1^flox alleles. Animals were grouping housed (2–4 mice/cage) on a 12-h light–dark cycled animal facility. All animal experiments utilized adult mice (between 10 and 16 weeks old) and analyzed with the experimenter blind to both genotype and treatment. All mouse protocols were approved by the Institutional Animal Care and Use Committee at the University of Texas Southwestern Medical Center at Dallas.

Drug treatment

Tamoxifen (Sigma) (500 mg/kg) in sunflower oil was administrated to adult mice by oral gavage. All other drugs were injected intraperitoneally (i.p.). Ketamine (7 mg/kg, Pfizer) was dissolved in saline and injected either 24 h or 1 week before the behavioral tests. The MEK inhibitor, SL327 (Sigma) was dissolved in DMSO (19 mg/ml) and injected (38 mg/kg) 1 h before saline/ketamine treatment³⁶. The volume of each single injection was 60–80 µl. Two hours before the killing, a single i.p. injection of Kainate (35 mg/kg) was given to adult mice to induce grade 4–5 seizures and only mice displaying the rearing behavior would be included in the experiment²⁴. For pulse-chase experiments, 4 doses of BrdU (5-Bromo-2’-deoxyuridine) were administered (100 mg/kg per injection, 2.5 h interval). To suppress adult neurogenesis, Temozolomide (TMZ, Sigma) was given to mice at 25 mg/kg (i.p., 2.5 mg/ml in saline), and the injections were performed on the first three days of a week for 4 weeks, followed by the forced swim test (see below) 4 weeks afterward⁴⁷ (Fig. 3a).

Immunohistochemistry and quantitative analyses

Mice were intracardially perfused with PBS followed by 2% paraformaldehyde (PFA) in PBS and the dissected brains postfixed in 4% PFA overnight at 4 degrees. Brains were then equilibrated in 30% sucrose and mounted in OCT (Fisher). Frozen sections were cut coronally at 18 µm. Immunofluorescence was performed as described previously^20,48. Sections were incubated with the primary antibodies in blocking solution (10% donkey serum and 0.4% Triton X-100 in PBS) at the following dilutions: NeuN (1 : 200, Millipore, ABN78), Doublecortin (DCX) (1 : 200, Santa Cruz, sc8066), GFAP (1:500, BD bioscience 556329), Ki67 (1 : 200,Thermo, RM9106), Calbindin (1 : 200, Swant, #300), β-galactosidase (1 : 200, Abcam, ab9361) followed by the incubation with the corresponding donkey secondary antibodies conjugated with Cy2, Cy3 or Cy5 (1 : 300, Jackson Immunoresearch) and DAPI (Vector Labs) for counterstaining. For the staining of p-AKT (1 : 500, Cell signaling 9271), p-ERK (1 : 500, Cell signaling 4370), p-S6 (1 : 500, Cell signaling 2211), biotin-conjugated donkey anti-rabbit was used as secondary antibody and the fluorescent signal was detected using a tyramide signal amplification (TSA) kit (Perkin Elmer) following the manufacturer’s instructions. For BrdU staining, sections were pretreated with 2 N HCl for 20 min to denature DNA for the exposure of BrdU antigen, followed by incubation with BrdU antibody (1 : 200, Abcam, ab6326) in blocking solution overnight. The representative images of immunofluorescence were taken from at least five animals.

Digital fluorescent images were obtained with a Nikon epifluorescence microscope and Zeiss LSM 710 confocal system. All representative confocal images are shown as a maximum intensity projection of a z-series stack acquired from 16 µm thick sections with a z-step of 2 µm. Every sixth coronal section from part of adult dentate gyrus (bregma: −2.46 to −1.34 mm) was used to assess neurogenesis in both hemispheres (10 sections per animal in each condition). Quantification of newborn neuron number/percentage (NenN+/DCX−/BrdU+ or NeuN+/DCX−/tdTOM) and DCX+ progenitors (DCX+/BrdU+ or DCX+/tdTOM) was performed on the orthogonal view of each confocal z-stack image for the precise determination of protein co-expression (total 50–60 BrdU+ or over 200 tdTOM+ cells were analyzed per animal), by using MetaMorph image analysis software (Molecular Devices)^20,48. Many of DCX+ immature neurons have very low NeuN expression and were counted as DCX+ progenitors. Fluorescent images of DCX, Ki67, BrdU or GFAP positive Cells were captured in both hemispheres and counted manually and blindly for the genotypes or treatments. Cell counts from eight sections were multiplied by 6 to estimate the total number in every dentate gyrus. To quantify EGR1 expression in newborn neurons, 20–30 BrdU+ cell per animal were analyzed for the triple positive cell number and their percentage in newborn neurons. For the quantification of the DCX+ cell with dendrites in TMZ experiments, cells with dendrites longer than the diameters of DCX labeled soma were counted on the confocal images with maximum intensity projection of a z-series stack, and at least 8 images were quantified for each animal in both conditions. For the analysis of dendritic morphology, biocytin+ neurons or tdTOM+ neurons with mostly intact dendritic branches were selected and 30 µm thick z-series of images were collected for the dendritic tracing by NeuroJ. The number of secondary/tertiary dendrites and branch points was counted manually²¹. Fluorescent confocal images of DCX and p-ERK were captured from 16 µm thick sections and analyzed with the single confocal z-stack planes (n = 4 mice for each treatment). For experiments that include both male and female mice, we attempted to have similar gender proportions, which are indicated for comparison.

Western blotting

The dentate gyrus and CA1 region were carefully dissected from four hippocampal slices per mouse (~ 1mm thick). Tissue samples were rapidly frozen and lysed in RIPA buffer (Thermo Fisher Scientific). Protein samples from at least three animals were used independently for immunoblotting with antibodies at the following dilutions: BDNF (1 : 200, Santa Cruz, sc546), p-TrkB (1 : 1000, Abcam, ab81288), p-AKT (1 : 1000, Cell signaling 9271), p-ERK (1 : 1000, Cell signaling 9101), p-S6 (1 : 1000, Cell signaling 2211), ERK (1 : 1000, Cell signaling 9102), β-Actin (1 : 2000, Santa Cruz, sc69879). Western lightning plus-ECL (Perkin Elmer) was used for signal detection, and each blot might be stripped and reprobed with different antibodies. Quantification of band intensity normalized to the β-actin band was performed using MetaMorph image analysis software (Molecular Devices)⁴⁸.

Acute dentate gyrus slice preparation

Three weeks after the tamoxifen induction, adult mice (Nestin-creER^T2; tdTOM) were deeply anesthetized and transcardially perfused with chilled (4 °C) dentate gyrus dissection buffer containing (in mM): 110 Choline Cl, 2.5 KCl, 1.3 KH₂PO₄, 25 NaHCO₃, 10 D-glucose, 0.6 Na Pyruvate, 1.3 Na Ascorbate at pH 7.4, 300 mOsm, and aerated with 95% O2/5% CO2, including 0.5 CaCl2, 7 MgCl2, and 5 Kynurenate acid. Transverse hippocampal slices (250 µm thickness) were obtained on a Leica VT1200S slicer, and then recovered for 30 min at 35 °C and for another 15 min at room temperature in artificial cerebrospinal fluid (ACSF) containing (in mM): 125 NaCl, 2.5 KCl, 1.3 KH₂PO₄, 25 NaHCO₃, 1.3 Na Pyruvate, 10 d-glucose, 1.3 Na Ascorbate, 2 CaCl₂, 1.3 MgCl₂ aerated with 95% O2/5% CO₂ to pH 7.4. A single slice was then transferred to a submersion chamber and perfused at 3 ml/min with aerated ACSF at 30 °C ready to be recorded.

Electrophysiology

Lineage-traced cells in the dentate gyrus were identified under visual guidance using IR-DIC optics and tdTomato fluorescence, followed by the whole-cell patch clamp recordings. The recordings were performed using glass pipettes (3–5MΩ) filled with intracellular solution (0.2 mM EGTA, 130 mM K-gluconate, 6 mM KCl, 3 mM NaCl, 10 mM HEPES, 4 mM ATP-Mg, 0.4 mM GTP-Na, and 14 mM phosphocreatine-Tris at pH 7.2 and 285 mOsm) supplemented with 0.5% biocytin (B4261; Sigma) for the labeling. All recordings were obtained with a MultiClamp 700B amplifier. Currents were filtered at 2 kHz, acquired and digitized at 10 kHz using Clampex 10.3 (Molecular Devices). Action Potentials (APs) were recorded in current-clamp mode and elicited by a series of current injections ranging from −20 to 200 pA with 5, 10, or 20 pA increments and 800 ms duration. Sodium and potassium currents were recorded in voltage-clamp in response to a series of voltage steps ranging from −60 mV to +60 mV at 10-mV increments and 200 ms duration. Sodium current was measured as the inward current. Delayed rectifier potassium currents (I _d) were measured 50 ms prior to the end of the current step. Fast potassium currents (I _A) were measured at the peak of outward current immediately after sodium currents and then subtracted by I _d. Spontaneous synaptic currents were recorded in voltage-clamp mode. In all voltage-clamp recordings, cells were clamped at −60 mV except during the voltage-step protocol. In all current-clamp recordings, recordings were made at the resting membrane potential or without any current injection. Series and input resistance were measured in a voltage-clamp mode with a 400 ms, −10 mV step from a −60 mV holding potential (filtered by 10 kHz, sampled at 50 kHz). Cells were accepted only if the series resistance was less than 30 MΩ and stable throughout the experiment.

Data analysis was performed in Clampfit 10.3 software (Molecular Devices). The action potential (AP) trace immediately above threshold was used to determine the delay of 1st spike as the length of time from the start of current steps to the peak of AP; to measure AP threshold as the corresponding voltage when there was the sharpest change of trace slope; to determine AP amplitude, half width, maximum velocity of rise and decay by using the “Statistics” function from the “Analyze” menu as peak amplitude, half-width, maximum rise and decay slope. AP frequency was obtained by dividing the maximum number of spikes during the current steps protocol with the step time duration (800 ms). Similarly, sodium and potassium currents were measured using the “Statistics” function. The biggest current was used. Spontaneous postsynaptic currents and spontaneous endplate currents were analyzed by using the Mini Analysis Program v6.0.7 (Synaptosoft). Traces were imported into the program, and baseline noise was measured by “measuring RMS noise” option in “Noise Analysis” menu. Four times the noise was used as the threshold for detection. Each individual event was carefully examined to avoid false positives. Statistics can be shown from the “Events” menus.

Behavior tests

All behavioral experiments were performed during the light cycle. All animals used for the tests were littermates with all possible genotypes. The age of the mice in all experimental groups was 10–16 weeks and the age difference in each experimental group is within 2 weeks in order to eliminate any potential age-related influence on neurogenesis. Male (70%) and female (~30%) animals were tested. Since separate analyses show no statistically significant gender difference in each group, both data sets were incorporated. Researchers were blind to animal genotype and treatment information during testing.

The forced swim test (FST) was performed as described previously^20,21. Since the test is sensitive to both conventional antidepressants and ketamine^8,49, it was used as the primary test for assessing the ketamine anti-depressive behavioral response in this study. Briefly, mice were placed in a 4 L glass beaker with 3 L water at 22–24 °C. Water was changed between subjects. All tests were recorded by a digital camcorder positioned on the side of the beaker. The videos were analyzed and scored by an experimenter blind to genotype/treatment and only the last 4 min of the total 6 min test was scored for immobility time. Immobility was defined as floating or remaining motionless except essential motions for keeping the head above the water. A decrease in immobility time indicates an antidepressant-like effect.

In the novelty-suppressed feeding test (NSFT), group-housed mice were deprived of food for 20 h prior to the test. Individual mice were placed in a 23 × 23 × 10 inch open field arena. Two or three pellets of food chow were placed in the center of the arena. The latency for each animal to approach and eat food was measured. Each test was terminated when the mouse first ate the food or when 10 min had elapsed without the mouse eating. Immediately following the NSFT, the amount of food consumed within 5 min in a normal housing cage was monitored as a control measure for appetite. Six days after NSFT, the same mice were subjected to the FST as an assessment of anti-depressive behavioral effect 1 week after the treatment.

In the learned helplessness test (LH), mice were individually placed on one side of a two-chamber shuttlebox (Med Associates) with the door closed for 1 h, receiving 120 shocks (0.35 mA for 2 s) with the unpredictable interval between shocks (18–44 s, average 30 s). This training was repeated for two days. On the test day, the door between the two chambers was raised at the onset of each shock and the shock ended either when the mouse stepped through the door or after 25 s. The number of escapes and the latency of each escape was recorded for 15 trials. Mice were not subjected to any other behavioral tests after LH.

Statistical analyses

All data are presented as mean ± SEM. Statistical analysis was done with GraphPad Prism or SPSS software. The D’Agostino & Pearson or Shapiro–Wilk normality test was first done on the data to determine whether it was a normal distribution. The sample size with continuous variables is calculated by SPSS. Statistical significance was defined as p < 0.05 using either a two-way ANOVA for comparisons among multiple groups (Supplementary Table 1) or an unpaired two-tailed t-test or the Mann–Whitney test for two groups of samples. Post hoc group multiple comparisons were performed with Turkey test. For two-way ANOVA with unequal sample size, the unweighted mean and type III Sum of Squares were calculated by SPSS. NS label in charts represents not significant in statistical analyses. One, two and three stars (*) in charts represent p-value < 0.05, < 0.01 and < 0.001, respectively.

Data availability

The data that support the findings of this study are available from the corresponding authors upon reasonable request.

References

Lopez, A. & Murray, C. The global burden of disease, 1990-2020. Nat. Med. 4, 1241–1243 (1998).
Article CAS PubMed Google Scholar
Morilak, D. & Frazer, A. Antidepressants and brain monoaminergic systems: a dimensional approach to understanding their behavioural effects in depression and anxiety disorders. Int. J. Neuropsychopharmacol. 7, 193–218 (2004).
Article CAS PubMed Google Scholar
Fagiolini, A. & Kupfer, D. J. Is treatment-resistant depression a unique subtype of depression? Biol. Psychiatry 53, 640–648 (2003).
Article PubMed Google Scholar
Trivedi, M. H. et al. Evaluation of outcomes with citalopram for depression using measurement-based care in STAR*D: implications for clinical practice. Am. J. Psychiatry 163, 28–40 (2006).
Article PubMed Google Scholar
Berman, R. M. et al. Antidepressant effects of ketamine in depressed patients. Biol. Psychiatry 47, 351–354 (2000).
Article CAS PubMed Google Scholar
Price, R. B., Nock, M. K., Charney, D. S. & Mathew, S. J. Effects of intravenous ketamine on explicit and implicit measures of suicidality in treatment-resistant depression. Biol. Psychiatry 66, 522–526 (2009).
Article CAS PubMed PubMed Central Google Scholar
Zarate, C. A. Jr et al. A randomized trial of an N-methyl-D-aspartate antagonist in treatment-resistant major depression. Arch. Gen. Psychiatry 63, 856–864 (2006).
Article CAS PubMed Google Scholar
Autry, A. E. et al. NMDA receptor blockade at rest triggers rapid behavioural antidepressant responses. Nature 475, 91–95 (2011).
Article CAS PubMed PubMed Central Google Scholar
Kavalali, E. T. & Monteggia, L. M. How does ketamine elicit a rapid antidepressant response? Curr. Opin. Pharmacol. 20, 35–39 (2015).
Article CAS PubMed Google Scholar
Duman, R. S. & Aghajanian, G. K. Synaptic dysfunction in depression: potential therapeutic targets. Science 338, 68–72 (2012).
Article ADS CAS PubMed PubMed Central Google Scholar
Li, N. et al. mTOR-dependent synapse formation underlies the rapid antidepressant effects of NMDA antagonists. Science 329, 959–964 (2010).
Article ADS CAS PubMed PubMed Central Google Scholar
Duman, R. S. & Li, N. A neurotrophic hypothesis of depression: role of synaptogenesis in the actions of NMDA receptor antagonists. Philos. Trans. R. Soc. Lond. B. Biol. Sci. 367, 2475–2484 (2012).
Article CAS PubMed PubMed Central Google Scholar
Lyons, D. M. et al. Stress coping stimulates hippocampal neurogenesis in adult monkeys. Proc. Natl Acad. Sci. USA 107, 14823–14827 (2010).
Article ADS CAS PubMed PubMed Central Google Scholar
Perera, T. D. et al. Necessity of hippocampal neurogenesis for the therapeutic action of antidepressants in adult nonhuman primates. PLoS ONE 6, e17600 (2011).
Article ADS CAS PubMed PubMed Central Google Scholar
Castren, E. & Rantamaki, T. The role of BDNF and its receptors in depression and antidepressant drug action: Reactivation of developmental plasticity. Dev. Neurobiol. 70, 289–297 (2010).
Article CAS PubMed Google Scholar
Sahay, A. & Hen, R. Adult hippocampal neurogenesis in depression. Nat. Neurosci. 10, 1110–1115 (2007).
Article CAS PubMed Google Scholar
Zhao, C., Deng, W. & Gage, F. H. Mechanisms and functional implications of adult neurogenesis. Cell 132, 645–660 (2008).
Article CAS PubMed Google Scholar
Snyder, J. S., Soumier, A., Brewer, M., Pickel, J. & Cameron, H. A. Adult hippocampal neurogenesis buffers stress responses and depressive behaviour. Nature 476, 458–461 (2011).
Article ADS CAS PubMed PubMed Central Google Scholar
Boldrini, M. et al. Antidepressants increase neural progenitor cells in the human hippocampus. Neuropsychopharmacology 34, 2376–2389 (2009).
Article CAS PubMed PubMed Central Google Scholar
Li, Y. et al. TrkB regulates hippocampal neurogenesis and governs sensitivity to anti-depressive treatment. Neuron 59, 399–412 (2008).
Article CAS PubMed PubMed Central Google Scholar
Li, Y., McKay, R. M., Riethmacher, D. & Parada, L. F. Neurofibromin modulates adult hippocampal neurogenesis and behavioral effects of antidepressants. J. Neurosci. 32, 3529–3539 (2012).
Article CAS PubMed PubMed Central Google Scholar
Park, H. & Poo, M. M. Neurotrophin regulation of neural circuit development and function. Nat. Rev. Neurosci. 14, 7–23 (2013).
Article CAS PubMed Google Scholar
Chen, J., Kwon, C. H., Lin, L., Li, Y. & Parada, L. F. Inducible site-specific recombination in neural stem/progenitor cells. Genesis 47, 122–131 (2009).
Article CAS PubMed PubMed Central Google Scholar
Waterhouse, E. G. et al. BDNF promotes differentiation and maturation of adult-born neurons through GABAergic transmission. J. Neurosci. 32, 14318–14330 (2012).
Article PubMed PubMed Central Google Scholar
Soumier, A., Carter, R. M., Schoenfeld, T. J. & Cameron, H. A. New hippocampal neurons mature rapidly in response to ketamine but are not required for its acute antidepressant effects on neophagia in rats. eNeuro 3; 10.1523/ENEURO.0116-15.2016 (2016).
Kee, N., Teixeira, C. M., Wang, A. H. & Frankland, P. W. Preferential incorporation of adult-generated granule cells into spatial memory networks in the dentate gyrus. Nat. Neurosci. 10, 355–362 (2007).
Article CAS PubMed Google Scholar
Jungenitz, T., Radic, T., Jedlicka, P. & Schwarzacher, S. W. High-frequency stimulation induces gradual immediate early gene expression in maturing adult-generated hippocampal granule cells. Cereb. Cortex 24, 1845–1857 (2014).
Article PubMed Google Scholar
Ivanova, A. et al. In vivo genetic ablation by Cre-mediated expression of diphtheria toxin fragment A. Genesis 43, 129–135 (2005).
Article CAS PubMed PubMed Central Google Scholar
Chen, J. et al. A restricted cell population propagates glioblastoma growth after chemotherapy. Nature 488, 522–526 (2012).
Article ADS CAS PubMed PubMed Central Google Scholar
Martinez-Canabal, A., Akers, K. G., Josselyn, S. A. & Frankland, P. W. Age-dependent effects of hippocampal neurogenesis suppression on spatial learning. Hippocampus 23, 66–74 (2013).
Article CAS PubMed Google Scholar
Sairanen, M., Lucas, G., Ernfors, P., Castren, M. & Castren, E. Brain-derived neurotrophic factor and antidepressant drugs have different but coordinated effects on neuronal turnover, proliferation, and survival in the adult dentate gyrus. J. Neurosci. 25, 1089–1094 (2005).
Article CAS PubMed Google Scholar
Scharfman, H. et al. Increased neurogenesis and the ectopic granule cells after intrahippocampal BDNF infusion in adult rats. Exp. Neurol. 192, 348–356 (2005).
Article CAS PubMed Google Scholar
Donovan, M. H., Yamaguchi, M. & Eisch, A. J. Dynamic expression of TrkB receptor protein on proliferating and maturing cells in the adult mouse dentate gyrus. Hippocampus 18, 435–439 (2008).
Article CAS PubMed PubMed Central Google Scholar
Luikart, B. W. et al. TrkB has a cell-autonomous role in the establishment of hippocampal Schaffer collateral synapses. J. Neurosci. 25, 3774–3786 (2005).
Article CAS PubMed Google Scholar
Numakawa, T. et al. BDNF function and intracellular signaling in neurons. Histol. Histopathol. 25, 237–258 (2010).
CAS PubMed Google Scholar
Lee, Y. S. et al. Mechanism and treatment for learning and memory deficits in mouse models of Noonan syndrome. Nat. Neurosci. 17, 1736–1743 (2014).
Article CAS PubMed PubMed Central Google Scholar
Vogel, K. S., Brannan, C. I., Jenkins, N. A., Copeland, N. G. & Parada, L. F. Loss of neurofibromin results in neurotrophin-independent survival of embryonic sensory and sympathetic neurons. Cell 82, 733–742 (1995).
Article CAS PubMed Google Scholar
Li, N. et al. Glutamate N-methyl-D-aspartate receptor antagonists rapidly reverse behavioral and synaptic deficits caused by chronic stress exposure. Biol. Psychiatry 69, 754–761 (2011).
Article CAS PubMed PubMed Central Google Scholar
Ming, G. L. & Song, H. Adult neurogenesis in the mammalian brain: significant answers and significant questions. Neuron 70, 687–702 (2011).
Article CAS PubMed PubMed Central Google Scholar
Klesse, L. J. & Parada, L. F. p21 ras and phosphatidylinositol-3 kinase are required for survival of wild-type and NF1 mutant sensory neurons. J Neurosci 18, 10420-10428 (1998).
Samuels, I. S., Saitta, S. C. & Landreth, G. E. MAP’ing CNS development and cognition: an ERKsome process. Neuron 61, 160–167 (2009).
Article CAS PubMed PubMed Central Google Scholar
Zhu, Y. et al. Ablation of NF1 function in neurons induces abnormal development of cerebral cortex and reactive gliosis in the brain. Genes Dev. 15, 859–876 (2001).
Article CAS PubMed PubMed Central Google Scholar
Sanchez-Ortiz, E. et al. NF1 regulation of RAS/ERK signaling is required for appropriate granule neuron progenitor expansion and migration in cerebellar development. Genes Dev. 28, 2407–2420 (2014).
Article PubMed PubMed Central CAS Google Scholar
Duric, V. et al. A negative regulator of MAP kinase causes depressive behavior. Nat. Med. 16, 1328–1332 (2010).
Article CAS PubMed PubMed Central Google Scholar
Ji, Y. et al. Acute and gradual increases in BDNF concentration elicit distinct signaling and functions in neurons. Nat. Neurosci. 13, 302–309 (2010).
Article CAS PubMed PubMed Central Google Scholar
Zanos, P. et al. NMDAR inhibition-independent antidepressant actions of ketamine metabolites. Nature 533, 481–486 (2016).
Article ADS CAS PubMed PubMed Central Google Scholar
Garthe, A., Behr, J. & Kempermann, G. Adult-generated hippocampal neurons allow the flexible use of spatially precise learning strategies. PLoS ONE 4, e5464 (2009).
Article ADS PubMed PubMed Central CAS Google Scholar
Ma, Z., Wang, J., Song, F. & Loeb, J. A. Critical period of axoglial signaling between neuregulin-1 and brain-derived neurotrophic factor required for early Schwann cell survival and differentiation. J. Neurosci. 31, 9630–9640 (2011).
Article CAS PubMed PubMed Central Google Scholar
Maeng, S. et al. Cellular mechanisms underlying the antidepressant effects of ketamine: role of alpha-amino-3-hydroxy-5-methylisoxazole-4-propionic acid receptors. Biol. Psychiatry 63, 349–352 (2008).
Article CAS PubMed Google Scholar

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Acknowledgements

We thank Lauren Peca and Yanjiao Li for technical support, and all members of the Parada laboratory for valuable discussions and suggestions. We also thank Drs Lisa Monteggia, and Yun Li for critical reading of this manuscript and insightful comments. This work was supported by The Excellence in Education Fund of the Southwestern Foundation, by the Kent Waldrep Foundation for Nerve Regeneration, by the Southwestern Ball Chair and by the Diana and Richard C. Strauss Chair in Developmental Biology at UT Southwestern Medical Center.

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Zilai Wang & Luis F. Parada
Present address: Brain Tumor Center & Program in Cancer Biology and Genetics, Memorial Sloan Kettering Cancer Center, 1275 York Ave, New York, NY, 10065, USA

Authors and Affiliations

Department of Developmental Biology & Kent Waldrep Center for Basic Research on Nerve Growth and Regeneration, University of Texas Southwestern Medical Center, Dallas, TX, 75390, USA
Zhenzhong Ma, Zilai Wang & Luis F. Parada
Department of Neuroscience, University of Texas Southwestern Medical Center, Dallas, TX, 75390, USA
Zhenzhong Ma & Jane E. Johnson
Department of Molecular Biology, University of Texas Southwestern Medical Center, Dallas, TX, 75390, USA
Tong Zang & Chun-Li Zhang
Department of Psychiatry, University of Texas Southwestern Medical Center, 5323 Harry Hines Blvd, Dallas, TX, 75390, USA
Shari G. Birnbaum

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Zhenzhong Ma
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Contributions

Z.M. and L.F.P. conceptualized the research and wrote the manuscript. Z.M. designed the experiments. Z.M., S.G.B., and Z.W performed molecular, cellular and behavioral studies. T.Z. and C-L.Z. performed electrophysiology experiments. J.E.J. provided reagents. Z.M. and T.Z. analyzed the data.

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Correspondence to Zhenzhong Ma or Luis F. Parada.

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Ma, Z., Zang, T., Birnbaum, S.G. et al. TrkB dependent adult hippocampal progenitor differentiation mediates sustained ketamine antidepressant response. Nat Commun 8, 1668 (2017). https://doi.org/10.1038/s41467-017-01709-8

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Received: 21 July 2017
Accepted: 06 October 2017
Published: 21 November 2017
DOI: https://doi.org/10.1038/s41467-017-01709-8

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