Dysfunction of the RAR/RXR signaling pathway in the forebrain impairs hippocampal memory and synaptic plasticity
© Nomoto et al; licensee BioMed Central Ltd. 2012
Received: 5 January 2012
Accepted: 8 February 2012
Published: 8 February 2012
Retinoid signaling pathways mediated by retinoic acid receptor (RAR)/retinoid × receptor (RXR)-mediated transcription play critical roles in hippocampal synaptic plasticity. Furthermore, recent studies have shown that treatment with retinoic acid alleviates age-related deficits in hippocampal long-term potentiation (LTP) and memory performance and, furthermore, memory deficits in a transgenic mouse model of Alzheimer's disease. However, the roles of the RAR/RXR signaling pathway in learning and memory at the behavioral level have still not been well characterized in the adult brain. We here show essential roles for RAR/RXR in hippocampus-dependent learning and memory. In the current study, we generated transgenic mice in which the expression of dominant-negative RAR (dnRAR) could be induced in the mature brain using a tetracycline-dependent transcription factor and examined the effects of RAR/RXR loss.
The expression of dnRAR in the forebrain down-regulated the expression of RARβ, a target gene of RAR/RXR, indicating that dnRAR mice exhibit dysfunction of the RAR/RXR signaling pathway. Similar with previous findings, dnRAR mice displayed impaired LTP and AMPA-mediated synaptic transmission in the hippocampus. More importantly, these mutant mice displayed impaired hippocampus-dependent social recognition and spatial memory. However, these deficits of LTP and memory performance were rescued by stronger conditioning stimulation and spaced training, respectively. Finally, we found that pharmacological blockade of RARα in the hippocampus impairs social recognition memory.
From these observations, we concluded that the RAR/RXR signaling pathway greatly contributes to learning and memory, and LTP in the hippocampus in the adult brain.
Retinoic acids (RAs) are biologically active metabolites of vitamin A, an essential nutrient factor [1–3]. Vitamin A-RA signaling pathways play essential roles in a wide range of biological functions such as reproduction, growth, differentiation, development, vision, and homeostasis of various tissues, including the brain [2, 4].
All-trans-RA and 9-cis-isomers of RA bind to their nuclear receptor, i.e., RA receptors (RARα, β, and γ) and retinoid × receptors (RXRα, β, and γ), which function as ligand-inducible transcription factors [4, 5]. RA binding to RAR and RXR, respectively, forms a heterodimer of RAR/RXR or a homodimer of RXR/RXR and regulates the transcription of target genes by binding to retinoic acid responsive elements in their promoter regions, thereby regulating various biological phenomena [4, 6].
RAR and RXR, especially RARα are highly expressed in a wide range of central nervous system tissues including the mature brain [7, 8]. Moreover, there is growing evidence that vitamin A-RA signaling pathways have an impact on higher brain function; furthermore, an impairment of these signaling pathways is implicated in the etiology of Alzheimer's disease and psychiatric disorders such as schizophrenia [9–15]. Indeed, recent studies using mice have shown that age-related memory deficits are associated with the hypo-function of vitamin A-RA signaling pathways and these deficits are restored by treatment with RA or supplementation of vitamin A [16, 17].
Importantly, deletion of the RARβ or RARβ/RXRγ genes leads to deficits in hippocampal synaptic plasticity, e.g., long-term potentiation (LTP) and long-term depression (LTD) . Similarly, vitamin A-deficient mice display impaired hippocampal LTP that is rescued by treatment with RA [19, 20]. These findings strongly suggest that the RAR/RXR signaling pathway plays critical roles in hippocampal LTP and LTD. However, the roles of the RAR/RXR signaling pathway in learning and memory have not been well characterized in the mature brain, especially in the hippocampus. Indeed, previous genetic studies have shown that mice lacking the RARβ or RARβ/RXRγ genes displayed deficits in motor coordination that made it difficult to estimate their learning and memory abilities . However, these studies suggested that loss-of-function of the RAR/RXR signaling pathway impairs spatial learning and memory . Additionally, these studies did not exclude the possibility that genetic depletion of the RAR/RXR genes leads to some developmental changes in the brain.
In the current study, we tried to understand the roles of the RAR/RXR signaling pathway in hippocampus-dependent learning and memory and in hippocampal synaptic plasticity. To do this, we generated conditional mutant mice in which the expression of a dominant-negative mutant of RARα could be induced in the forebrain using a tetracycline-dependent transcription factor, and performed electrophysiological experiments and hippocampus-dependent memory tasks using these transgenic mice. Furthermore, we examined the effects of pharmacological inhibition of RARα in the hippocampus on memory performance.
Generation of dnRAR mice
We first generated two lines (H02 and H06) of mutant mice that express dnRAR fused with an HA-tag at the N-terminus under the control of a tetracycline-responsive element (TRE)-dependent promoter (TRE-dnRAR mice) . These mutant mice were crossed with transgenic mice that express tTA in the forebrain under the control of the αCaMKII promoter, which displays strong activity in the forebrain including the hippocampus, cortex, and amygdala (CaMKII-tTA mouse) , generating 2 lines of CaMKII-tTA/TRE-dnRAR double transgenic mice (dnRAR H02 and H06 mice).
To decrease the effects of dnRAR expression on the development of the forebrain, transgenic mice and wild-type (WT) littermates were treated with Dox until they were 8 weeks old and they were then housed without Dox-treatment to induce the expression of dnRAR (transgene OFF - transgene ON; OFF/ON; Figure 1B). For the control groups, dnRAR H06 mice were treated with Dox throughout their lifetime (transgene OFF; OFF-dnRAR mice) and OFF/ON-dnRAR H06 mice were treated again with Dox for 4 weeks following withdrawal of Dox for 4 weeks (transgene OFF-transgene ON-transgene OFF; OFF/ON/OFF-dnRAR mice; Figure 1B).
We next performed expression analysis of dnRAR in the forebrain and hippocampus of dnRAR H02 and H06 mice. Northern blot analysis using a specific probe for the 3'-untranslated region (UTR) of dnRAR mRNA revealed that dnRAR mRNA was expressed in the forebrain and hippocampus of the 2 OFF/ON double transgenic lines (Figure 1C). Importantly, dnRAR H02 mice displayed higher levels of dnRAR mRNA expression than the dnRAR H06 mice. Consistently, Western blotting using an anti-HA antibody showed the expression of dnRAR in the hippocampus of OFF/ON-dnRAR H06 mice (Figure 1D). Importantly, the expression of dnRAR was not detectable in the hippocampus of OFF/ON/OFF-dnRAR H06 mice. These observations indicated that the dnRAR mice express dnRAR in the forebrain, including the hippocampus, in a Dox-dependent manner.
We finally examined the effects of dnRAR expression on RAR/RXR-dependent gene expression in the forebrain. To do this, we analyzed the expression levels of RARβ, a target gene of RAR/RXR [1, 28], in the forebrain and hippocampus using Northern blotting and quantitative RT-PCR (qRT-PCR) (Figure 1E, F, respectively). One-way analysis of variance (ANOVA) of the Northern blotting results revealed a significant effect of genotype on RARβ expression (F (2,21) = 5.953, p < 0.05; Figure 1E). The post hoc Newman-Keuls test revealed that the expression levels of RARβ mRNA in the forebrain of OFF/ON-dnRAR H02 and H06 mice were significantly lower than in WT mice (p < 0.05). Additionally, dnRAR-H06 mice displayed slightly lower expression levels of RARβ mRNA than dnRAR-H02 mice, although this difference was not statistically significant. Similarly, qRT-PCR showed that OFF/ON-dnRAR H06 mice displayed significantly lower expression levels of RARβ mRNA in the hippocampus than WT mice (p < 0.05; Figure 1F). Importantly, this decreased expression of RARβ mRNA in the hippocampus was rescued when these OFF/ON mice were treated again with Dox for 4 weeks (OFF/ON/OFF-dnRAR mice; OFF/ON/OFF vs. OFF/ON, p < 0.05; OFF/ON/OFF vs. WT, p > 0.05), indicating that the down-regulation of RARβ mRNA is dependent on the expression of dnRAR. Collectively, these observations indicated that the expression of dnRAR decreases RARβ mRNA levels in the forebrain, including the hippocampus, suggesting that dnRAR expression leads to dysfunction of the RAR/RXR signaling pathway in these brain regions. Our results indicate that the expression levels of dnRAR in the OFF/ON-dnRAR H06 mice are sufficient to downregulate RAR/RXR-target gene expression; therefore, the subsequent electrophysiological and behavioral analyses were performed using the dnRAR-H06 transgenic line.
Basal synaptic transmission and LTP in the hippocampus of dnRAR mice
Previous studies have shown that genetic deletion of one or two RAR/RXR subtypes impaired LTP in the CA1 region of the hippocampus . To examine the effects of the impaired RAR/RXR signaling pathway on synaptic plasticity, we recorded extracellular field potentials in the CA1 region of hippocampal slices from OFF/ON-dnRAR H06 mice and WT littermates.
We next analyzed paired-pulse facilitation (PPF), a presynaptic form of short-term synaptic plasticity, in dnRAR H06 mice (Figure 2B). PPF was induced by a pair of afferent fiber stimulations at short intervals (50, 100, 200, or 300 ms). dnRAR H06 mice showed comparable PPF at each inter-pulse interval compared with WT mice, suggesting that the probability of release of the neurotransmitter glutamate from the presynaptic terminal is normal in dnRAR H06 mice (each interval, p > 0.05). We also analyzed post-tetanic potentiation (PTP), which is a presynaptic phenomenon (Figure 2C) . PTP was induced by conditioning stimulation (100 Hz, 1 s) in the presence of D-APV (50 μM), an NMDA receptor antagonist. The magnitude of PTP following stimulation was comparable between dnRAR and WT mice, suggesting that short-term plasticity induced by conditioning stimulation was normal in dnRAR mice (p > 0.05 at each time point).
Next, we analyzed LTP in dnRAR H06 mice. LTP was induced using a single high-frequency stimulation (one 100 Hz, 1 s train; Figure 2D and 2E). It is important to note that the stimulus strength was adjusted to obtain similar initial EPSP slope values (0.10-0.15 mV/ms) in each experiment because dnRAR H06 mice displayed impaired AMPA receptor-mediated input-output relationships compared with WT mice (Figure 2A). WT mice displayed significant synaptic potentiation following high-frequency stimulation compared with their baseline responses (p < 0.05; Figure 2D), indicating that single conditioning stimulation was sufficient to induce LTP in the hippocampal slices from WT mice. Conversely, dnRAR H06 mice also displayed significant LTP compared with their baseline responses (p < 0.05). However, the magnitude of LTP in these mutant mice was significantly lower at 51-60, 111-120, and 171-180 min following the induction of LTP compared with WT littermates (p < 0.05; Figure 2E), although the magnitude was comparable at 21-30 min between dnRAR H06 and WT mice (p > 0.05), suggesting that dnRAR H06 mice failed to maintain LTP even though LTP was induced normally. These observations indicated that dnRAR H06 mice displayed impaired LTP in the CA1 region of the hippocampus.
We examined whether stronger conditioning stimulation rescues the impaired LTP observed in the dnRAR H06 mice. To do this, LTP was induced by four high-frequency stimulations (four 100 Hz, 1 s trains at 5 min intervals; Figure 2F and 2G). WT and dnRAR H06 mice displayed significant LTP compared with their baseline responses (p < 0.05). In contrast to the results from single conditioning stimulation, dnRAR H06 mice displayed a comparable magnitude of LTP at each time point compared with WT mice. These observations suggest that strong conditioning stimulation rescued the impaired LTP observed in dnRAR H06 mice. However, we could not exclude the possibility that strong conditioning stimulation led to saturated levels of LTP, thereby masking differences in the magnitude of LTP between WT and dnRAR H06 mice.
We finally examined short-term potentiation (STP; Figure 2H). STP was induced by using shorter conditioning stimulation (100 Hz for 100 ms) than that used to induce LTP (100 Hz for 1 s). The magnitude of STP after induction was comparable between dnRAR H06 mice and WT littermates (p > 0.05). These observations suggest that dnRAR H06 mice displayed normal STP.
Taken together, our observations confirmed previous observations that dysfunction of the RAR/RXR signaling pathway results in impaired hippocampal LTP and extended these findings by demonstrating that this dysfunction also leads to an impaired AMPA receptor-mediated synaptic response. However, we could not exclude the possibility that impaired AMPA receptor-mediated EPSPs observed in dnRAR H06 mice contributed to the failure of LTP maintenance.
Impaired social memory in dnRAR mice and its rescue by stronger training
Our finding that the impaired LTP observed in OFF/ON-dnRAR H06 mice was rescued by stronger conditioning stimulation raised the possibility that stronger training could also rescue the impaired STM in OFF/ON-dnRAR H06 mice. To examine this, the mice were tested using a stronger training protocol in which they were exposed to a juvenile mouse for 3 min during the training and test sessions (Figure 3B) . In contrast to the results shown above, one-way ANOVA revealed no significant effect of genotype (F(1,16) = 0.006, p > 0.05). Consistently, WT and OFF/ON-dnRAR H06 mice displayed a significant decrease in social investigation time during the test compared with the training, indicating that both groups formed STM. These observations indicated that stronger training rescued the impaired STM observed in dnRAR H06 mice.
We next examined the effects of dnRAR expression on the formation of long-term memory (LTM; Figure 3C). The mice were exposed to a juvenile mouse for 3 min during the training and test sessions, which were performed 24 h apart. In this experiment, OFF-dnRAR H06 mice that were administered Dox throughout their lifetime were also tested as a control group to clarify the effect of dnRAR expression. One-way ANOVA revealed an effect of group (F(2,68) = 7.992, p < 0.05). OFF/ON-dnRAR H06 mice displayed a significantly worse recognition index than the WT and OFF-dnRAR H06 mice (p < 0.05), which displayed comparable recognition indices (p > 0.05). Consistently, the control groups (p < 0.05), but not OFF/ON-dnRAR H06 mice (p > 0.05), displayed significant decreases in social investigation time during the test compared with the training, indicating that the control groups formed LTM, while dnRAR H06 mice did not. These observations indicated that dnRAR H06 mice display impaired LTM in a dnRAR expression-dependent manner.
On the basis of our observations in the STM experiment, we examined whether a stronger training protocol rescues the impaired LTM observed in dnRAR H06 mice (Figure 3D). To do this, we used a spaced training protocol because a previous study demonstrated that the impaired LTM observed in mutant mice was rescued by a spaced, but not massed, training protocol . The mice were trained with exposure to a juvenile mice for 3 min twice with an interval of 0 min (massed training), 10 min, or 1 h (spaced training), and 24 h later, they were tested with exposure to the same juvenile mouse for 3 min (test). We assessed the recognition indices, i.e., the ratio of the social investigation time during the test relative to the first exposure during training. Two-way ANOVA with the duration of the interval (0 and 10 min, and 1 h) and genotype revealed an effect of genotype (F(1,67) = 11.930, p < 0.05), suggesting that, similar with the result shown in Figure 3C, dnRAR mice displayed impaired LTM. Consistently, the post hoc Newman-Keuls test revealed that massed-trained OFF/ON-dnRAR H06 mice displayed a significantly worse recognition index than the other groups (p < 0.05), indicating that massed-trained dnRAR mice exhibited significantly impaired LTM. However, spaced-trained dnRAR mice (10 min or 1 h) displayed a comparable recognition index with the other groups of WT mice (p > 0.05), suggesting that these groups of spaced-trained mutant mice exhibited normal LTM. Consistently, although all groups displayed significant decreases in social investigation time during the test compared with the first exposure during training (p < 0.05), massed-trained OFF/ON-dnRAR H06 mice displayed a significant, but small, decrease in their social investigation time. These observations indicated that the impaired LTM observed in OFF/ON-dnRAR H06 mice was rescued by spaced, but not massed, training with an interval of 10 min-1 h.
We also performed a social recognition test using another transgenic line (dnRAR H02 mice) that displays higher expression levels of dnRAR (Figure 3E). The mice were trained and then tested 24 h later with exposure to a juvenile mouse for 3 min. Consistent with the result for dnRAR H06 mice, one-way ANOVA revealed a significant effect of genotype (F(1,22) = 23.568, p < 0.05). OFF/ON-dnRAR-H02 mice showed a significantly worse recognition index than WT mice (p < 0.05). Consistently, WT, but not OFF/ON-dnRAR H02, mice exhibited a significant decrease in social investigation time during the test compared with training (p > 0.05). These observations confirmed that the expression of dnRAR in the forebrain leads to impaired social recognition memory.
Taken together, our observations indicated that dnRAR mice have impaired ST- and LT-social recognition memories. Importantly, these memory impairments are rescued by stronger training.
Impaired spatial memory in dnRAR mice and its rescue by stronger training
On the basis of the observations in the social recognition task, it is possible that spaced training could rescue the impaired memory performance observed in dnRAR H06 mice. To examine this, the mice were trained with 2 trials at 1 h intervals per day for 7 days (Figure 4B). In contrast to the previous results, two-way repeated ANOVA revealed a significant effect of time, but not genotype (genotype, F(1,25) = 2.872, p > 0.05; time, F(6,150) = 46.768, p < 0.05), indicating that both groups of mice displayed a comparable improvement of memory performance as both groups showed decreases in escape latency with training days. Consistently, the results of the probe test revealed that WT and OFF/ON-dnRAR H06 mice spent significantly more time in the TQ compared with the other quadrants, indicating that both groups formed spatial memory. These results indicated that the impaired spatial memory observed in OFF/ON-dnRAR H06 mice was rescued by spaced training. Collectively, these observations indicated that OFF/ON-dnRAR H06 mice have a deficit in spatial memory, but this deficit is rescued by stronger training, and confirmed our findings in the social recognition task.
It is important to note that WT and OFF/ON-dnRAR H06 mice showed normal locomotor activity and anxiety-related behaviors (time spent in the center of field) in the open field test (Additional file 1, Figure S1). Furthermore, OFF/ON-dnRAR H06 mice displayed normal swim speed (Additional file 2, Figure S2) and social investigation time during the training session in social recognition test (Figure 3), compared to WT mice. These observations strongly suggest that memory impairments observed in dnRAR mice does not attribute to abnormal locomotor and/or emotional behaviors such as social and anxiety-related behaviors.
Pharmacological loss-of-function of hippocampal RARα impairs social recognition memory
In this study, we characterized the roles of the RAR/RXR signaling pathway in the forebrain during learning and memory. To do this, we generated conditional mutant mice in which the expression of dnRAR was induced only in the forebrain of adult mice using a tetracycline-dependent transcription factor expression system. These mutant mice induced dnRAR expression in a Dox-dependent manner and down-regulated RARβ gene expression, a target gene of RAR/RXR, in a dnRAR expression-dependent manner, suggesting that these mutant mice only display a dysfunction of the RAR/RXR signaling pathway in the forebrain when dnRAR is expressed. Similarly with previous findings, these dnRAR mice displayed impaired LTP, especially the maintenance of LTP in the hippocampus; however, this deficit of LTP was rescued by stronger stimulation. Furthermore, we observed an impaired AMPA receptor-mediated synaptic response in dnRAR mice. These findings suggest that the dysfunction of the RAR/RXR signaling pathway impairs synaptic transmission as well as potentiation in the hippocampus. Conversely, dnRAR mice displayed deficits in ST- and LT-social recognition memory without an effect on immediate memory (see Figure 3D). Interestingly, these impairments of STM and LTM in the dnRAR mice were rescued by stronger or spaced training, respectively. Consistently, dnRAR mice displayed normal spatial learning and memory in the Morris water maze when they were spaced trained, but not when they were massed trained. Furthermore, pharmacological inhibition of RARα in the hippocampus impaired social recognition memory. These behavioral observations suggest that the RAR/RXR signaling pathway plays critical roles in hippocampus-dependent memory. Taken together, our observations strongly suggest that the RAR/RXR signaling pathway is required for synaptic transmission and plasticity and learning and memory in the forebrain, especially the hippocampus.
Memory consolidation is a process that generates LTM [35–37]. Previous studies have shown that the inhibition of gene expression blocks the formation of LTM without affecting STM [38–40]. Indeed, the activation of CREB-mediated transcription plays an essential role in memory consolidation and LTP [33, 39]. In this study, we showed that dysfunction of the RAR/RXR signaling pathway impairs STM and LTM. These observations suggest that RAR/RXR play distinct roles from CREB in hippocampus-dependent memory; it is unlikely that RAR/RXR greatly contribute to memory consolidation via learning-induced RAR/RXR-mediated transcription, as CREB does. Indeed, our finding that loss of RAR/RXR function impairs not only LTP but also the AMPA receptor-mediated synaptic response raises the possibility that RAR/RXR contribute to leaning/memory via basal synaptic transmission as well as long-term plasticity.
Interestingly, we observed that RAR/RXR dysfunction impaired the hippocampal LTP induced by a single conditioning stimulus and hippocampus-dependent social and spatial memories. However, stronger stimulation (four conditioning stimuli) and stronger or spaced training rescued these impairments in LTP and memories, respectively. The similarity of the observations at the cellular and behavioral levels strongly suggests the importance of the RAR/RXR signaling pathway in the hippocampus for both plasticity and learning and memory. Furthermore, this importance is supported by our observations that the pharmacological inhibition of RARα function in the hippocampus blocked the formation of social recognition memories. Further studies are required to examine the correlation between synaptic plasticity and learning/memory ability in the hippocampus of dnRAR mice, and the roles of RAR-mediated long-term plasticity in memory performance.
Recent reports have shown that RARα is present in the dendrites located in the hippocampus and induces the translation of GluA1 in a RA-dependent manner, resulting in the increased membrane insertion of GluA1 [41, 42]. Interestingly, this regulation of GluA1 by RARα is independent of transcriptional regulation [42, 43]. In the absence of RA, cytoplasmic RARα directly binds with GluA1 mRNA localized in dendrites via its C-terminal F-domain and represses its translation . In the presence of RA, RA binding to RARα releases the GluA1 mRNA that is trapped by RARα, leading to the translational activation of GluA1 . The dominant-negative mutant of RARα used in this study lacks the C-terminus, including the F-domain that is required for its interaction with GluA1 mRNA . Therefore, it is possible that the dnRAR used in this study not only inhibits RAR/RXR-mediated transcription but also affects the translational regulation of GluA1. dnRAR might block the RA-dependent release of GluA1 mRNA in dendrites by trapping RA and inhibiting the translational activation of GluA1 mRNA, resulting in the down-regulation of AMPA-mediated synaptic transmission.
The findings in this and other studies showed that the dysfunction of RAR/RXR leads to impairments of memory and LTP in the hippocampus [18–20]. Conversely, previous studies have suggested that the age-related down-regulation of RAR/RXR-mediated gene expression is implicated in the cognitive decline of aged mice [16, 17]. Importantly, these studies demonstrated that the administration of RA alleviates the down-regulated expression of RA-target genes in the hippocampus, age-related deficits in hippocampal LTP, and memory performance. Furthermore, the administration of RA prevents the deposition of Aβ and rescues memory deficits in a transgenic mouse model of Alzheimer' disease . Taken together, these observations raise the possibility that the RAR/RXR signaling pathway positively regulates memory performance and, moreover, that the activation of this signaling pathway improves learning and memory. Further studies are required to examine the effects of gain of RAR/RXR function on learning and memory by the genetic enhancement of RAR/RXR.
A previous genetic study showed that the deletion of the RARβ or RARβ/RXRγ genes leads to disrupted LTP and LTD in the CA1 region of the hippocampus without affecting basal synaptic transmission . In contrast, our results indicated that dysfunction of the RAR/RXR signaling pathway by the expression of dnRAR impairs the maintenance, but not induction, of CA1-LTP and the AMPA receptor-mediated synaptic response. The differences between these two studies may reflect distinct roles of RAR/RXR subtypes in synaptic transmission and potentiation in the hippocampus [6, 46]. Additionally, there is a possibility that the protocols used to induce LTP contributed to the different findings of these two studies.
In summary, we found that dysfunction of the RAR/RXR signaling pathway leads to the down-regulation of RARβ expression and impairment of AMPA-mediated synaptic transmission and LTP in the hippocampus and hippocampus-dependent social recognition and spatial memories. More interestingly, stronger conditioning stimulation and training rescued these impairments of LTP and memory performance, respectively. Furthermore, we showed that blocking the function of RARα in the hippocampus disrupted social recognition memory. These observations strongly suggested that the RAR/RXR signaling pathway in the hippocampus plays critical roles in synaptic plasticity and memory performance.
Materials and methods
Mice were housed in cages of 5 or 6, maintained on a 12 h light/dark schedule, and allowed ad libitum access to food and water in their home cages. All of the experiments were conducted during the light phase of the cycle in an illuminated testing room according to the Guide for the Care and Use of Laboratory Animals, Japan Neuroscience Society and Tokyo University of Agriculture. All of the experiments were conducted blind to the treatment condition of the mouse. Animal behavior was recorded using a video camera.
Generation of the dominant-negative RARα mutant (dnRAR) lacking the C-terminal region of RARα (aa 403-462) was performed as described previously . To generate dnRAR cDNA, 2 separate fragments of the dnRAR cDNA (nucleotides 1-438 and 433-1206) were amplified by reverse transcription-polymerase chain reaction (RT-PCR) using mouse brain cDNA as a template with the following primers: 1/438 primers (sense, gggggatccagatctatggccagcaatagcagttc; antisense, ggggaattcctgcagccggcagtactggc); 433/1209 primers (sense, gggggatccctgcagaaatgtttcgacgt; antisense, ggggaattcacgcgtaagctttca gatctccatcttcaatg; the termination codon to generate dnRAR is underlined). The resulting RT-PCR fragments were subcloned into the Bam HI-Eco RI sites of pBluescript II (SK+) (Agilent Technologies, CA, USA), generating pBS-dnRAR. The Bgl II-Hind III fragment encoding dnRAR from pBS-dnRAR was ligated with the Bgl II-Hind III fragment from pTRE-dnBMAL1 , generating pTRE-dnRAR.
Generation of transgenic mice
pTRE-dnRAR was digested with Mlu I, and transgenic mice were generated by injecting the purified insert into the pronuclei of C57BL/6N zygotes. TRE-dnRAR founders were crossed with C57BL/6N mice (Charls River Japan, Kanagawa, Japan). These founders were crossed with mice (CaMKII-tTA) expressing the tTA transgene under the control of the αCaMKII promoter , generating double-transgenic mice (dnRAR TgM). Genotyping was performed by Southern blot analysis using specific probes derived from the 0.5 kbp Not I-Nde I fragment containing the TRE-promoter region from pcisTRE  and the 0.6 kbp Eco RI-Hind III fragment containing the tTA-coding region from pcDNA3-TetR-KRAB .
Administration of doxycycline
TRE promoter-dependent transgene expression was regulated using the animal's drinking water containing 1 μg/mL doxycycline (Dox) (Sigma, MO, USA) dissolved in 5% sucrose to mask the bitter taste of Dox.
Northern blot analysis was performed as described previously [39, 47]. Total RNA was prepared as described previously [39, 47]. To generate a specific probe for TRE promoter-dependent transcripts, the 0.3 kbp Hind III-Xba I fragment containing the 3'-UTR from pTRE-dnRAR was used. The filters were hybridized with a specific probe for the 3'-UTR and then re-hybridized with GAPDH cDNA as an internal control. qRT-PCR was performed as described previously . qRT-PCR was performed on an ABI PRISM 7000 using the Power SYBR Green PCR Master Mix (Applied Biosystems, CA, USA) according to the manufacturer's protocol. The reaction was first incubated at 50°C for 2 min, then at 95°C for 10 min, followed by 40 cycles of 95°C for 15 s and 60°C for 1 min. All measurements were performed in triplicate. The levels of GAPDH mRNA were used to normalize the relative expression levels of target mRNA. The PCR primers used were as follows (5' to 3'): RARβ forward, tcctggatcaatgccacctc; RARβ reverse, acacgctggactgtgctct; GAPDH forward, atggccttccgtgttcctac; and GAPDH reverse, gcctgcttcaccaccttctt. Western blot analysis using a rabbit polyclonal anti-HA antibody (1:1000; Santa Cruz Biotechnology, CA, USA) and a mouse monoclonal anti-α-tubulin antibody (1:1000; Santa Cruz Biotechnology, CA, USA) was performed as described previously [48, 49]. Equal protein loading was confirmed by reprobing with the anti-α-tubulin antibody. The protein bands were detected using the ImmunoStar LD system (Wako, Osaka, Japan) according to the manufacturer's protocol, and the chemiluminescence signals were analyzed with the ChemiDoc XRS detection system and QuantityOne software (Bio-Rad Laboratories, CA, USA).
Before the commencement of the behavioral experiments, the mice were individually handled for 2 min each day for 1 week. Individual mice were used for all experiments.
Social recognition test
The social recognition test was performed as described previously [32, 33]. Adult mice were placed into individual plastic cages in an experimental room under dim light. The cages were identical to those in which mice were normally housed (plastic, 30 × 17 × 12 cm). After a period of 60 min, a juvenile mouse was placed into a cage with a subject for a training trial that lasted for 1.5 min (see Figure 3A) or 3 min (see Figures 3B, C, E, 5A). The duration of social investigation behavior exhibited by the adult mouse was determined using a hand-held stopwatch. Social investigation was measured as described previously . Memory was reassessed at 2 h or 24 h later by recording the length of the investigation time exhibited by the subject to the same juvenile (test). To evaluate the differences in the ability to form social memory between the groups of mice, we calculated a recognition index, i.e., the ratio of the duration of the second and first investigation times. When massed or spaced training was performed, the subjects were trained with 2 trials lasting 3 min at intervals of 0 min (massed-training) and 10 min, 1 h (spaced training) on the first trial day. Memory was reassessed at 24 h after the training as described above. The recognition index was calculated as the ratio of the social investigation time during the test relative to the first exposure during training.
Morris water maze test
The Morris water maze test was performed as described previously [33, 40, 51]. The mice were trained with 2 trials at intervals of 1 min (see Figure 4A) or 1 h (see Figure 4B) per day for 7 days. The mice were tested at approximately the same time everyday. In the probe test at 24 h after 7 d of training, the platform was removed, and the mice were allowed to swim for 60 s. We measured the time that the mice spent in each quadrant.
Surgery for drug microinfusion
Surgery was performed as described previously [51–54]. Under Nembutal anesthesia and using standard stereotaxic procedures, stainless steel guide cannulae (22 gauge) were implanted into the dorsal hippocampus (-1.8 mm, ± 1.8 mm, -1.9 mm). Ro41-5253 (Ro41) (Enzo Life Sciences, NY, USA), an RARα-selective antagonist, was dissolved in dimethyl sulfoxide (DMSO) (Wako, Osaka, Japan), and then dissolved in vehicle solution (VEH) [artificial CSF (ACSF)] with a final DMSO concentration of 0.01%. Micro-infusions into each brain region (0.5 μL) were made at a rate of 0.25 μL/min. The injection cannula was left in place for 2 min after the infusion.
Electrophysiology was performed as described previously [30, 55]. All experiments were performed to compare dnRAR mice with WT mice in a blind fashion using littermates. Three- to 5-month-old dnRAR and WT mice were decapitated under deep halothane anesthesia, and both hippocampi were removed. Hippocampal slices (400-μm thick) were cut with a Vibratome tissue slicer and placed in a humidified interface-type chamber for at least 1 h. A single slice was then transferred to the recording chamber, which was maintained at 25°C, and submerged beneath a continuously perfusing medium (119 mM NaCl, 2.5 mM KCl, 1.3 mM MgSO4, 2.5 mM CaCl2, 1.0 mM NaH2PO4, 26.2 mM NaHCO3, and 11 mM glucose) that had been saturated with 95% O2 and 5% CO2. All perfusing solutions contained picrotoxin (100 μM) to block gamma-aminobutyric acid A receptor (GABA-A-R)-mediated inhibitory synaptic responses. Field potential recordings were made using a glass electrode filled with 3 M NaCl and placed in the stratum radiatum of the hippocampal CA1 region.
To evoke synaptic responses, a bipolar stimulating tungsten electrode was placed in the stratum radiatum, and Schaffer collateral/commissural fibers were stimulated at 0.1 Hz (test pulses). An Axopatch 200B amplifier (Molecular Devices, Sunnyvale, USA) was used, and the signal was filtered at 1 kHz and digitized at 10 kHz, and stored on a personal computer. The stimulus strength was adjusted so that it gave rise to AMPA receptor-mediated EPSPs with a slope value between 0.10 and 0.15 mV/ms. For the analysis of EPSPs, we measured their early rising phase to avoid contamination from voltage-dependent components as much as possible. Each data point represents the averaged slope value for 1 min that was normalized to the baseline slope value. For LTP recording, LTP was induced using 1 or 4 high-frequency stimulations (one 100 Hz, 1 s train or four 100 Hz, 1 s trains at 5 min intervals, respectively). For STP recording, STP was induced using a single high-frequency stimulation (one 100 Hz, 100 ms train). To record the input-output relationships, D-2-amino-5-phosphonovaleric acid (D-APV, 25 μM) was present to block N-methyl-D-aspartate receptor (NMDA-R)-mediated synaptic responses. A low concentration of 6-cyano-7-nitro-quinoxaline-2,3-dione (CNQX, 1 μM) was also present to partially block alpha-amino-3-hydroxy-5-methyl-4-isoxazole propionate receptor (AMPA-R)-mediated synaptic responses because the fiber volleys were usually much smaller than the EPSPs. This enables more accurate measurements of the input-output relationships, since the presence of low concentrations of CNQX reduces the nonlinear summation of field EPSPs when strong stimulus strengths are used. For the measurement of PPF, afferent fibers were stimulated twice at intervals of 50, 100, 200, and 300 ms in the presence of D-APV (25 μM). For PTP recordings, PTP was induced using a single high-frequency stimulation (one 100 Hz, 1 s train) in the presence of D-APV (50 μM). Data were collected using Clampex 5.0 and analyzed with pClamp 9.0 software. Picrotoxin and D-APV were purchased from Sigma (MO, USA) and CNQX was purchased from Tocris Cookson (Avonmouth, UK).
Data were analyzed with ANOVA. One-way ANOVA analysis followed by the post hoc Newman-Keuls comparison was used to analyze the effects of genotype, time, and drug. Two-way ANOVA analysis followed by the post hoc Newman-Keuls comparison was used to analyze the effects of genotype, time, and duration of the interval. All values in the text and figure legends represent the mean ± SEM. A paired t test was used to analyze the differences in the social investigation times within each group between training and test in the social recognition test, and to analyze the differences of the time spent in the TQ compared with the other quadrants in the Morris water maze test. Student's t test (two-tailed, unpaired) was used to determine whether there was a significant difference in the means between two sets of data in the electrophysiological experiments.
List of abbreviations
α-calcium/calmodulin-dependent protein kinase II.
S.K. was supported by Grant-in-Aids for Scientific Research (B) (23300120 and 20380078) and (C) (18580129), Grant-in-Aids for Scientific Research on Priority Areas -Molecular Brain Science- (18022038 and 22022039), High Technology Research and from the Ministry of Education, Culture, Sports, Science, and Technology, Japan, Core Research for Evolutional Science and Technology (CREST), Japan, a Research Grant for Nervous and Mental Disorders from the Ministry of Health, Labor, and Welfare, Japan, 4th Itsuu Laboratory Research Grant, Japan, The Sumitomo Foundation, Japan and the Takeda Science Foundation, Japan.
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