Abstract
Most excitatory synapses in the brain form on dendritic spines. Two-photon uncaging of glutamate is widely utilized to characterize the structural plasticity of dendritic spines in brain slice preparations in vitro. In the present study, glutamate uncaging was used to investigate spine plasticity, for the first time, in vivo. A caged glutamate compound was applied to the surface of the mouse visual cortex in vivo, revealing the successful induction of spine enlargement by repetitive two-photon uncaging in a magnesium free solution. Notably, this induction occurred in a smaller fraction of spines in the neocortex in vivo (22%) than in hippocampal slices (95%). Once induced, the time course and mean long-term enlargement amplitudes were similar to those found in hippocampal slices. However, low-frequency (1â2âHz) glutamate uncaging in the presence of magnesium caused spine shrinkage in a similar fraction (35%) of spines as in hippocampal slices, though spread to neighboring spines occurred less frequently than it did in hippocampal slices. Thus, the structural plasticity may occur similarly in the neocortex in vivo as in hippocampal slices, although it happened less frequently in our experimental conditions.
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Introduction
Most excitatory synapses in the brain form on dendritic spines. The volume of dendritic spines is tightly correlated with the functional expression of glutamate receptors in the young hippocampal slice preparations1,2,3,4,5,6 and in the adult mouse neocortex in vivo7. Spine volume changes accompany long-term potentiation and depression of synapses in hippocampal slices8,9,10,11,12. Such volume changes may lead to the generation and elimination of spines13,14,15,16,17,18,19 as well as impaired structural plasticity which ultimately leads to pathological neuronal circuitry18,20,21.
Two-photon uncaging of caged glutamate compounds is the only method that reliably stimulates single spines1. Furthermore, it is widely used to characterize structural spine changes in vitro. Spine enlargement is most robustly induced by uncaging glutamate in the absence of external magnesium (Mg2+), such that N-methyl-d-aspartic acid (NMDA) receptors are maximally activated8,10,22,23,24,25,26. Spine shrinkage is induced by low-frequency uncaging11,12,27. However, assessing spine plasticity with two-photon uncaging has never been applied in vivo because of the technical difficulties associated with uncaging in a living animal. The characteristics of structural plasticity in vivo are therefore unknown in the adult mouse neocortex.
We previously established a glutamate uncaging method in vivo in which a caged glutamate compound was applied to the surface of the brain. This allowed the compound to spread to the superficial extracellular space of the neocortex by passive diffusion7. The present study extends this work to assess the structural plasticity of dendritic spines, for the first time, in vivo.
Results
In vivo spine enlargement
A compound for two-photon uncaging of glutamate (Methods) was applied to single spines of the tuft dendrites of layer 5/6 pyramidal neurons in the visual cortex of adult mice (nâ=â18) in vivo7. A yellow fluorescent protein (YFP)-expressing mouse line (H) or green fluorescent protein (GFP)-expressing mouse line (M), in which a subset of pyramidal neurons are labelled in a layer 5/6 selective manner, were used. Mice were anesthetized with urethane and xylazine and placed under a microscope objective lens using an imaging chamber that was firmly attached to the mouse skull (Fig. 1A). To activate NMDA receptors effectively, the recording chamber was superfused with artificial cerebrospinal fluid containing no magnesium (Mg2+) ions. Caged glutamate was thereafter superfused (Fig. 1A, Supplementary Fig. 1A). Spine head volume (VH) fluctuations before uncaging were quantified as coefficients of variation (CVs) (Supplementary Fig. 1B). The CV of in vivo neocortex spines was 15%âÂąâ16% (meanâÂąâstandard deviation [SD]; 227 spines), compared to 21% in hippocampal slices8, demonstrating a similar stability of our recording conditions as in slices.
Spine enlargement was induced by two-photon glutamate uncaging, which was repeated 60 times at 1âHz in close proximity to the spine heads (Fig. 1B,C). Volume changes varied among individual spines; however, the averaged time course revealed a transient increment phase followed by a stable plateau phase (Fig. 1D). For spines with >30% enlargement, the peak enlargement (10â30âmin) and sustained phase of enlargement (>60âmin) were 109%âÂąâ24% (the meanâÂąâthe standard error of the mean: 16 spines/10 dendrites/10 mice) and 61%âÂąâ20%, respectively. These values were significantly different (Wilcoxon test; pâ=â0.028) and ranged similarly but less than those of CA1 pyramidal neurons (203%âÂąâ37% and 75%âÂąâ20%) in slices8. Enlargements lasting more than 30âmin occurred in eight of 16 enlarged spines (Fig. 2A) and were confined to stimulated spines (Figs 1D and 2B). The onset of enlargement was so rapid that volume increments were significant even at the first recording time point following uncaging (2âmin vs. â30â0âmin; by Wilcoxon signed rank test; pâ=â0.0016). The time-to-peak of the enlargement (~10âmin) was longer than that in young hippocampal slices (<1âmin). However, there was no significant difference among the amplitudes of enlargement at the three-time points after uncaging (2, 6 and 10âmin; by two-way ANOVA [pâ=â0.36]). Thus, spine enlargement in the neocortex in vivo exhibited a rapid and transient enlargement, similar to what occurred in hippocampal slices8.
Enlargement was recorded in a small fraction of spines (22% of 74 spines/20 dendrites/18 mice; Fig. 2A) as compared to the fraction recorded in the hippocampal slices (approximately 95%)8. In spines without enlargement (ÎVH <30%), average enlargement was negligible (â0.6%âÂąâ2.5%) (Fig. 1D). Less frequent spine enlargement did not seem to be due to technical reasons, as enlargement was induced mostly in one spine (0â4 spines; average, 0.8 spine) of those that were simultaneously stimulated (1â7 spines; average, 3.7 spines), unlike in slices8. This conclusion was further supported quantitatively by the observation that the enlargement amplitudes of stimulated spines were no correlated with the distance of the spine from another spine that exhibited significant enlargement (Fig. 2C), despite only enlarged spines (ÎVH >30%) being selected. We selected small spines (Fig. 2D) in which enlargement would be most pronounced in slice culture8. Enlargements were not correlated with spine depth or mouse age (Supplementary Fig. S2A,B), though only enlarged spines (ÎVH >30%) were selected.
Spine shrinkage in vivo
A solution containing a physiological concentration (1âmM) of Mg2+ was used to induce spine shrinkage27. Several spines on a dendrite were simultaneously stimulated with low-frequency two-photon glutamate uncaging (2.8 spines/dendrite average, 1â2âHz for 10â15âmin) (Fig. 3A). Stimulated spines exhibited as large of volume reductions (Fig. 3A,B, spine âS1â) over a gradual time course (Fig. 3C) as hippocampal slices11,27. We found that 35% of stimulated spines shrunk (âÎVH >30%, 15 of 43 spines/17 dendrites/8 mice) and that the mean amplitude at 20â50âmin was 19%âÂąâ4% (nâ=â43, medianâ=â17.5, interquartile rangeâ=â1.5:37.4), similar to that found in the young hippocampal slices (23%âÂąâ7%, nâ=â8)7. Furthermore, the shrinkage was persistent (>80âmin) in most (73%) spines (Fig. 4A) and was absent when the NMDA receptor antagonist APV was added to the perfusion solution (Figs 3C and 4B).
Spine shrinkage spread to neighboring spines, which also occurred in hippocampal slice culture samples11,27. We calculated an average spine volume of the stimulated spines and neighboring spines 20â50âmin from the onset of stimulation (Fig. 4C) and found that the spread of spine shrinkage was only significant in spines proximal to (<3 Îźm) those stimulated. Only 13% of spines within 3 Îźm of a stimulated spine exhibited shrinkage (âÎVStimulated >30%; Fig. 4D). Interestingly, spines with greater shrinkage tended to display less spread (Fig. 4D). Thus, the spread of spine shrinkage was less frequent in the adult neocortex in vivo than in young hippocampal slices in which shrinkage spread to 71% of spines within 3âÂľm and to 38% of spines within 7âÂľm of a stimulated spine11,27.
We found that the prestimulation spine volume was weakly and non-significantly correlated with spine shrinkage (Supplementary Fig. S3A). Spine retraction also occurred during spine shrinkage (Supplementary Fig. S3B,C)11; however, spine shrinkage was non-significantly correlated with retraction (ÎSpine length; Supplementary Fig. S3C). We did not observe any interspine distance dependency on the induction of spine shrinkage (Supplementary Fig. S4A). Spine shrinkage was also insignificantly correlated with dendritic depth (Supplementary Fig. S4B).
Discussion
In the current study, we present evidence for the successful induction of spine enlargement and shrinkage by uncaging glutamate in the adult mouse neocortex in vivo28. The essential features of this plasticity were similar to those reported previously in the hippocampal slices8. For enlargement, a rapid transient phase and sustained enlargement was noted, which was confined to stimulated spines. Shrinkage, however, occurred gradually and spread to neighboring spines.
A major difference between in vivo adult mouse neocortex changes here and those that occurred in hippocampal slice preparations previously8 was the success rate for the induction of spine enlargements (22% and 95%, respectively). This may have been due to differences in tissue age or other factors between the neocortex in vivo and the hippocampal slices. Additionally, difficulty in controlling concentrations of Mg2+ ions, the usage of anesthesia, types of neurons, parts of dendrites, and other technical reasons may have led to differences between the two paradigms. Importantly, once enlargement was induced, amplitude and persistence were similar between cortex and young hippocampal preparations. Moreover, the diversity cannot be simply explained by technical issues, as even one stimulated spine showed enlargement, however, other simulatneously stimulated neighboring spines did not, despite exposed to the same uncaging stimuli (Fig. 2C). Critically, we were able to determine that glutamate uncaging did in fact occur, as the induction of shrinkage was similar in hippocampal slice preparations (34â38%). These suggest some spine enlargement heterogeneity among neocortical spines in vivo.
As seen in the hippocampal slices, the spread of spine shrinkage to neighboring spines was also found in the neocortex11. However, neighboring spine shrinkage occurred less in neocortex than in young hippocampus. It should be noted, however, that shrinkage spread was dependent on the stimulation protocol, even in the same preparations. Spread was also more pronounced during spike-timing dependent plasticity (STDP)11 but negligible when low frequency (0.1âHz) uncaging was paired with a 200âms depolarization12. Thus, it is possible that such spread may be more extensive in vivo during STDP, which may help competition for neighboring plasticity11 and the removal of clustered spines29,30,31,32,33,34.
Thus, the two-photon in vivo uncaging technique used here led to a quantitative difference in the structural plasticity of dendritic spines in the adult neocortex in vivo as compared to that which occurred in hippocampal slice culture preparations. This supports the notion that the cortex is slower to learn than the hippocampus35. Although the expression of synaptic molecules is highly variable from spine to spine36, the molecular basis of this heterogeneity in enlargement requires further investigation.
Methods
Surgical procedures
All animal procedures were approved by the Animal Experiment Committee of the University of Tokyo (Tokyo, Japan). Procedures were conducted in accordance with the University of Tokyo Animal Care and Use Guidelines. Surgical procedures were performed as described previously7. In brief, we anesthetized adult mice expressing YFP or GFP in a subset of neurons: Thy1 YFP in the H line [YFP-H] or GFP in the M line [GFP-M]. Eighteen mice, aged 148âÂąâ129 days (meanâÂąâthe SD), were used for enlargement experiments (17 YFP-H mice; one GFP-M mouse) (Supplementary Fig. S2B). Eight mice, aged 70âÂąâ19 days, were used for shrinkage experiments (five YFP-H mice; three GFP-M mice) (Supplementary Fig. S4C). Mice were anesthetized with intraperitoneal injections of urethane and xylazine at 1.2âg/kg body weight and 7.5âmg/kg body weight, respectively, which were supplemented with subcutaneous administration of the analgesic ketoprofen (20âmg/kg body weight). A steel plate with a recording chamber was attached to the skull with cyanoacrylate glue such that the recording chamber was positioned just above the visual cortex (3.0âmm posterior, 2.5âmm lateral to the bregma)37. The plate was then tightly fixed to the metal platform. We then removed the skull using a pair of forceps and a dental drill, which was fixed to a stereotaxic instrument (Narishige, Tokyo, Japan). The dura mater was carefully removed using fine forceps and a microhook to minimize any pressure applied to the surface of the brain. We then placed a semicircular glass coverslip to cover approximately one-half of the exposed brain surface (Fig. 1A). The coverslip was fixed using either dental acrylic (Fuji-Lute BC; GC Corp., Tokyo, Japan) or a stainless steel wire. Mice were supplied with humidified oxygen gas and warmed to 37â°C with a heating pad (FST-HPS; Fine Science Tools Inc., North Vancouver, Canada) during all surgical procedures.
Two-photon in vivo imaging and uncaging
In vivo two-photon imaging and uncaging were conducted using an upright microscope (BX61WI; Olympus, Tokyo, Japan) equipped with a FV1000 laser scanning microscope system (Olympus) and a water-immersion objective lens (LUMPlanFI/IR 60X with a numerical aperture of 0.9; Olympus). The system included two mode-locked femtosecond-pulse titanium-sapphire lasers (MaiTai; Spectra Physics, Mountain View, CA, USA), one set to 720ânm for uncaging1 and the other to 980ânm for imaging. Each light path was connected to the microscope via an independent scan head and acousto-optic modulator. For 3-D reconstruction of dendrite images, 21â40 XY images separated by 0.5 Îźm were stacked by summing fluorescence values at each pixel. 4-Methoxy-7-nitroindolinyl (MNI)-glutamate or 4-carboxymethoxy-5,7-dinitroindolinyl (CDNI)-glutamate was custom-synthesized by the Nard Institute Ltd. (Amagasaki, Japan) or purchased from Tocris Bioscience (Bristol, UK) and perfused through the recording chamber via artificial cerebral spinal fluid (ACSF).
In vivo enlargement of dendritic spines
For in vivo spine enlargement experiments, the cortical surface was first superfused with magnesium-free ACSF (ACSF without Mg2+) containing 125âmM NaCl, 2.5âmM KCl, 3âmM CaCl2, 0âmM MgCl2, 1.25âmM NaH2PO4, 26âmM NaHCO3, 20âmM glucose, and 10âÂľM tetrodotoxin (Nacalai, Kyoto, Japan). This solution was bubbled with 95% oxygen and 5% carbon dioxide for approximately 30âÂąâ15âmin (meanâÂąâthe SD; 20 dendrites). The bathing solution was then changed to ACSF without Mg2+ containing 20âmM MNI-glutamate or 10âmM CDNI-glutamate and 200âÎźM Trolox (Sigma-Aldrich, St. Louis, MO, USA), which diffused into the cortical extracellular space approximately 15âmin before the uncaging experiments. Two-photon uncaging was aimed at the tip of the spines and repeated 60 times at 1âHz. The power of the uncaging laser was typically set to 10âmW for 0.6âms. We expected that transient currents similar to miniature excitatory-postsynaptic currents were elicited approximately at this laser power; however, we did not change power levels according to cortical depth7.
For each experiment, 2â8 spines (average, 4.6 spines) were stimulated along a dendrite. We studied 52 spines/15 dendrites/14 mice with MNI-glutamate and 22 spines/5 dendrites/4 mice with CDNI-glutamate. The enlargement success rates were 25% and 13%, respectively. The solution was pooled in a small reservoir (2âmL) (Fig. 1A). Pure water was constantly added (after empirically determining its flow rate) to the reservoir to maintain an osmotic pressure in the solution of approximately 320âmOsm/kg. The solution was warmed to 37â°C in the chamber with circulating hot water (Fig. 1A). All physiological experiments were conducted at 37â°C.
In vivo shrinkage of dendritic spines
For all spine shrinkage experiments, the cortical surface was superfused with ACSF containing 2âmM CaCl2 and 1âmM MgCl2. The solution was then changed before uncaging experiments to ACSF, which contained 200âÎźM of Trolox and a caged compound (i.e., 20âmM MNI-glutamate or 10âmM CDNI-glutamate). We studied 38 spines/15 dendrites/7 mice with MNI-glutamate and 5 spines/2 dendrites/1 mice with CDNI-glutamate. The success rate of shrinkage was 37% and 25%, for MNI-glutamate and CDNI-glutamate, respectively. Repetitive stimulation was conducted at 1â2âHz for 10â15âmin at a laser power similar to that used for enlargement (~10âmW).
As a control, stimulation was delivered in the presence of 50âmM d-2-amino-5-phosphonovaleric acid (APV), an NMDA receptor antagonist with MNI-glutamate.
Spine volume analyses
Spine head volumes were estimated from the total fluorescence intensity of spines by summing the fluorescence values of stacked images in 3-D using Image-J software (NIH, Bethesda, Maryland, USA), as reported previously7. When images contained axon fibers that overlapped with target dendrites at different image depths, the spine head volume in the dendrite was calculated by partially summing the fluorescence values of five sequential Z-images by taking the moving average of the image stack along the Z-plane. This was done to avoid axonal fibers. Because dendritic spines are near the diffraction limit of a two-photon microscope, partially summed values (2-Οm range in the Z-direction) were used to reflect spine volumes. Thus, the maximum value of Z-moving average images allowed for good approximation of total Z-summed stacked images.
Dendritic spines exhibit spontaneous fluctuations in fluorescence because of spontaneous morphological changes, motility, and measurement errors13. To determine spine volume fluctuations, we calculated the CV of in vivo images before glutamate uncaging (14.7%âÂąâ16.1% for 227 spines in the enlargement condition and 12.5%âÂąâ7.9% for 196 spines in the shrinkage condition). We set fluctuation limit values with a baseline of two CVs (i.e., 30% for enlargement data; 25% for shrinkage data) and discarded data when fluctuations exceeded this limit. Stimulated and neighboring spines with prestimulation fluctuations over this limit were discarded due to instability. For spine volume analyses, average spine volumes during the 10â30âmin (for enlargement) and 20â50âmin (for shrinkage) following stimulation were calculated and to indicate any differences from the baseline volume.
Spine length analysis
To determine spine length before and after stimulation, the length between the tip of the spine and the edge of the dendrite of interest was measured on Z-stack images (Supplementary Fig. S3B).
Statistical analysis
All data are presented as meanâÂąâstandard error of the mean (n indicates the number of spines), unless otherwise stated. Statistical tests of spine outcomes were conducted using Excel-Statistics software (Social Survey Research Information Co. Ltd., Tokyo, Japan). Differences from baseline values or between values were analyzed using the Wilcoxon signed-rank test (Figs 1D, 2B, 4BâD and S3B). Delays in the enlargement peak were analyzed via a two-way ANOVA (Fig. 1D). Spread of spine shrinkage was analyzed via a one-way ANOVA, followed by Tukeyâs post hoc multiple comparison testing (Fig. 4D). Pearsonâs product-moment correlation coefficients were calculated for scatter plots (Figs 2C,D, S2A,B, S3A,B and S4AâC). The significance of a correlation coefficient was determined via t-test. Differences between mean values for the two groups were analyzed using the Mann-Whitney rank-sum test (Fig. S5A).
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Acknowledgements
We wish to thank C. Maeda, M. Ogasawara, H. Ohno, Y. Sakata, K. Tamura, M. Nakajima, C. Matsubara, and T. Sasaki for their technical assistance. We also wish to thank N. Ichinohe for helpful discussion and support. This work was supported by Grants-in-Aids for Science Research (S) (26221011 to H.K.), Scientific Research (C) (18K06497 and 26430005 to J.N. and 2640290 to N.T.), Scientific Research in Innovative Areas (26111706 to J.N. and 16H06396 to S.Y.) and the âNetwork Joint Research Center for Materials and Devicesâ Cooperative Research Program (20171030 to J.N.), World Premier International Research Center Initiative support (to HK) from JSPS, CREST (JPMJCR1652 to H.K.) from JST, and the Strategic International Research Cooperative Program (SICP), Brain/MIND, and Strategic Research Program for Brain Sciences projects (17dm0107120h0002) from AMED (to H.K.).
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J.N. and H.K. are co-corresponding authors and designed the study; J.N. conducted most imaging experiments; A.N., H.U., T.H., S.Y. and N.T. assisted with some imaging experiments and with data analysis; J.N. and H.K. wrote the manuscript. All authors contributed to the editing.
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Noguchi, J., Nagaoka, A., Hayama, T. et al. Bidirectional in vivo structural dendritic spine plasticity revealed by two-photon glutamate uncaging in the mouse neocortex. Sci Rep 9, 13922 (2019). https://doi.org/10.1038/s41598-019-50445-0
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DOI: https://doi.org/10.1038/s41598-019-50445-0
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