Rett syndrome is a neurological disorder caused by mutation of the X-linked MECP2 gene. Mice lacking functional Mecp2 display a spectrum of Rett syndrome-like signs, including disturbances in motor function and abnormal patterns of breathing, accompanied by structural defects in central motor areas and the brainstem. Although routinely classified as a neurodevelopmental disorder, many aspects of the mouse phenotype can be effectively reversed by activation of a quiescent Mecp2 gene in adults. This suggests that absence of Mecp2 during brain development does not irreversibly compromise brain function. It is conceivable, however, that deep-seated neurological defects persist in mice rescued by late activation of Mecp2. To test this possibility, we have quantitatively analysed structural and functional plasticity of the rescued adult male mouse brain. Activation of Mecp2 in ∼70% of neurons reversed many morphological defects in the motor cortex, including neuronal size and dendritic complexity. Restoration of Mecp2 expression was also accompanied by a significant improvement in respiratory and sensory-motor functions, including breathing pattern, grip strength, balance beam and rotarod performance. Our findings sustain the view that MeCP2 does not play a pivotal role in brain development, but may instead be required to maintain full neurological function once development is complete.
Despite these pervasive defects, activation of a silenced Mecp2 allele in ∼80% of neurons after the onset of Rett syndrome-like signs reverses observed defects in both males and females (Guy et al., 2007). Reversibility appears to question the straightforward categorization of Rett syndrome as a neurodevelopmental disorder, as it suggests that MeCP2 deficiency during brain development does little lasting damage. A conservative interpretation might be, however, that reversal is superficial, meaning that underlying neurological defects persist in the ‘reversed’ mice. Phenotypic characterization by Guy et al. (2007) used semi-quantitative observational scoring for survival, gait, breathing, tremor, mobility and general condition (an exception was quantitatively robust reversal of defective hippocampal long-term potentiation). Here, we ask whether underlying features of brain morphology and sensory-motor function are rectified by late activation of Mecp2. We find that activation in ∼70% of neurons leads to significant improvement in almost all features, suggesting that phenotypic reversal is profound.
Materials and methods
Mecp2Stop/+ mice in which the endogenous Mecp2 allele is silenced by a targeted stop cassette (Mecp2tm2Bird, Jackson Laboratories Stock No. 006849) were crossed with hemizygous CreESR transgenic mice (CAG-Cre/ESR1*, Jackson Laboratories Stock No. 004453) to create experimental cohorts (Guy et al., 2007). Animals were bred on an inbred C57BL6/J background for neuronal morphology experiments. As breeding performance of Mecp2+/− animals is extremely poor on a C57BL6 inbred background, a breeding strategy of crossing C57BL6/J/CBA F1 animals and using the F2 offspring was adopted to facilitate the generation of large cohorts of mice for functional studies (behavioural and respiratory phenotyping). The genotype of the mice was determined by polymerase chain reaction (Guy et al., 2007). Mice were housed in groups with littermates, maintained on a 12-h light/dark cycle and provided with food and water ad libitum. Experiments were carried out in accordance with the European Communities Council Directive (86/609/EEC) and a project licence with local ethical approval under the UK Animals (Scientific Procedures) Act (1986).
Immunoblotting, polymerase chain reaction and Southern blots
Protein extracts for western blot analysis were prepared from snap-frozen brains that had been hemisected prior to freezing. Half brains were homogenized in a Dounce homogenizer in 750 μl ice-cold NE1 buffer [20 mM HEPES pH 7.9, 10 mM KCl, 1 mM MgCl2, 0.1% Triton X-100, 0.5 mM DTT, 20% glycerol, protease inhibitor cocktail (Roche)]. Samples were treated with 750 U Benzonase® (Sigma) for 15 min at room temperature. An equal volume of 2× loading buffer was added (125 mM Tris–Cl pH 6.8, 20% glycerol, 0.01% bromophenol blue, 2% β-mercaptoethanol) and the samples were vortexed, snap-frozen and boiled for 3 min.
Proteins were resolved by sodium dodecyl sulphate polyacrylamide gel electrophoresis and transferred to polyvinylidene fluoride membrane. Membranes were hybridized with a monoclonal antibody recognizing the C-terminus of MeCP2 (Sigma, M6818) and developed by quantitative infrared imaging (LI-COR Odyssey®, LI-COR Biosciences). Intensity of protein bands was quantified using LI-COR Odyssey® software.
Recombination of the Mecp2Stop allele was quantified as described previously (Guy et al., 2007) using the remaining half of each snap-frozen brain. When brains were to be used for Golgi–Cox staining, the front and rear portions of the brain were removed by coronal cuts for Southern analysis, before the central portion including the cortex was processed further.
Scoring of symptoms
Mice were observed and scored on a weekly basis for a number of symptoms arising from MeCP2 deficiency. These weekly assessments of cardinal Rett syndrome-like features generated a semi-quantitative measure of symptom status. Each of six signs (mobility, gait, hindlimb clasping, tremor, breathing and general condition) was scored as 0 (absent or as wild-type), 1 (symptom present) or 2 (symptom severe) as previously described (Guy et al., 2007). The aggregate score was used to determine when animals should commence tamoxifen treatment or be culled for humane reasons.
Tamoxifen (Sigma) was dissolved by sonication in corn oil (Sigma) at a concentration of 20 mg/ml aliquoted and stored at −20°C until required. Tamoxifen (100 mg/kg) was administered via intraperitoneal injection at an injection volume of 5 ml/kg body weight. A treatment regime of one injection of tamoxifen per week for 3 weeks followed by four daily injections on consecutive days in the fourth week was employed. For behavioural studies tamoxifen treatment was initiated once all animals had completed the initial behavioural screens (see below) and Stop/Cre lines displayed a group mean of 5/6 according to the severity scale of symptoms (see above). Animals for neuronal morphology and respiratory phenotyping were individually monitored and tamoxifen treatment started once the aggregate symptom score was at least 6. Wild-type controls were treated with tamoxifen in parallel with their littermates.
Golgi–Cox staining was performed using the FD Rapid GolgiStain kit (FD NeuroTechnologies). Male mice (age 9–21 weeks, Supplementary Fig. 1) were killed by cervical dislocation and brains rapidly removed, rinsed briefly in water and processed according to the manufacturer’s protocol, and sections were cut at 240 μm thickness on a cryostat. Pyramidal neurons from layer II/III of primary motor cortex (M1) were observed by an investigator blind to the genotype under a Nikon Eclipse E400 microscope and reconstructed on a 2D plane using a drawing tube under the ×40 objective lens. To ensure relative neuron completeness, cells were selected that were located close to the centre of the section and had pyramidal cell morphology with the primary apical dendritic trunk orientated in line with the plane of the section. Analysis was limited to a 220 μm radius, and cells with significant processes cut at the surface of the section were excluded from the analysis. Despite the most distal aspects of the dendritic arbor not being sampled with this approach, the method nevertheless allows the comparison of salient features of dendritic morphology in randomly sampled neurons from both genotypes and treatment groups before or following tamoxifen treatment. Branching was studied by Sholl analysis (Kishi and Macklis, 2004; McNair et al., 2010). For spine density analysis, segments of secondary oblique dendrites in hippocampal area CA1 (chosen due to the homogenous defined synaptic input and non-tapering dendrites), were reconstructed using ×100 oil immersion lens and the number of spines per unit length calculated (McNair et al., 2010). Morphological data were initially evaluated using unpaired t-tests and a secondary analysis conducted by ANOVA with Tukey’s posthoc test where appropriate. For Sholl analysis, groups were compared using a repeated measures two-way analysis of variance (ANOVA) with Tukey’s posthoc analysis.
Changes in respiratory frequency (mean ± SD) were recorded in vivo during periods of quiet restfulness by using whole body plethysmography (Buxco Electronics Inc.; Elphy software, INAF, CNRS). Respiratory baseline parameters were established for each mouse on three sequential days prior to tamoxifen treatment and again on three sequential days ∼5 weeks after the end of treatment.
The plethysmographic chamber (700 ml) was connected to a differential pressure transducer (Model DP103-4, Validyne Engineering), which measured pressure fluctuations within the closed chamber relative to a reference chamber of the same volume. During each 2 min recording session the chamber was hermetically sealed and temperature was continuously recorded and maintained between 27 and 28°C. Data from each 2 min recording were analysed using Spike 2 (Cambridge Instruments).The breath by breath analysis to determine baseline frequency and variability was performed on data recorded during periods of quiet wakefulness and excluded periods of apnoea (cessation of breathing, more than three missed breaths), hyperpnoea (rapid breathing) and movement. The number of sigh-like breaths was counted in each recording. Each mouse (Wild-type/Cre n = 11; Stop/Cre n = 10) was exposed to the protocol three times before and after tamoxifen treatment and the results of these sessions averaged. Data were statistically evaluated using two-way ANOVA followed where appropriate (P < 0.05) by Tukey’s posthoc test.
A typical experiment consisted of an initial assessment of the mice to define early mild symptoms at 5–6 weeks of age followed by tamoxifen treatment and retesting 5–6 weeks after treatment in the same protocols (Supplementary Figs 2 and 3). The low survival rate in Stop mice precluded retesting after treatment (no gene rescue) so that behavioural assessment was performed on two cohorts of male mice of Stop and Stop/Cre genotype and only survivors that completed the protocols pre- and 5–6 weeks post-treatment are considered. Cohort 1 (Wild-type/Cre n = 25; Stop/Cre n = 17) was tested in sequence for grip strength, on the rotarod, balance beams and CatWalk (see below). Cohort 2 (Wild-type/Cre n = 7; Stop/Cre n = 9) performed a short swim test.
The forelimb grip strength was determined using a grip-strength meter (Ugo Basile). Each mouse grasped the trapeze and upon gentle pulling of the tail, maximal grip strength was automatically recorded. Each animal performed two trials (intertrial interval 2 min).
An automated 4-lane accelerating RotaRod (TSE) was used to examine motor learning and motor coordination. Testing (pre- and post-treatment) consisted of four trials per day for two consecutive days with intertrial intervals of 2–3 min. For each trial, the mouse was placed on the rotating rod (1 rpm). The rod was accelerated from 1 to 45 rpm over the trial time of 5 min. Trials were terminated when animals fell off the rod or the maximum time was achieved. Lanes were allocated following a Latin square design to counterbalance for both rod position and time of testing.
Sensory-motor coordination was tested using balance beams (50 cm length; 28, 11 or 5 mm cross-section; 30% incline). Each mouse was given two trials per beam. Latency to traverse the beam was scored and averaged. Failure to traverse the beam during the allotted time terminated the trial and the maximum time (30 s) was recorded. As for all behavioural tests, apparatus was wiped with 70% ethanol between animals.
Gait analysis was performed on walking mice using the CatWalk (Noldus; version 7.1). Five trials per mouse with a maximum of 10 s to traverse the glass plate were administered. Data recorded include paw position, timing, pressure and dimensions of each footfall, which enabled calculation of stride length and paw distance.
The swim test was performed using an open-field water maze (150 cm diameter). Mice were released facing the wall of the pool and allowed to swim for 30 s after which time they were removed and returned to their home cages. The swim trajectory and speed of the mouse were recorded and tracked by an overhead video camera and tracking software Anymaze (Ugo Basile).
Data handling and analysis
For all behavioural data, Gaussian distribution was confirmed, before group means for each genotype and time point (pre- and post-treatment) were analysed by two-way ANOVAs followed, where appropriate, by Bonferroni posthoc tests using Prism 5.0 (Graphpad). Alpha was always set to 0.05. For simplicity, only reliable differences are indicated.
Silencing and rescue of MeCP2 expression in Mecp2Stop/y; CreESR mice
Expression of Mecp2 was interrupted by the insertion of a Stop cassette within intron 2 (Guy et al., 2007). Previous analysis did not detect MeCP2 protein in Mecp2lox–Stop/y,Cre-ER (Stop/y,Cre) mice. To more rigorously test for low-level expression of the Mecp2Stop allele, we carried out quantitative western blotting on protein from Stop/y males (n = 4). The results of replicate experiments showed that MeCP2 is expressed at ∼2.5% of the wild-type level in Stop/y male brains (Fig. 1A). Analysis of Stop/y males at different ages and with varying aggregate scores showed no correlation between the level of residual MeCP2 protein and the severity of symptom progression. For example, compare pair 1/2 (least severe, 1.1% wild-type level) with pair 7/8 (most severe, 3.8% wild-type level). Although a small number of Stop/y animals in this study showed extended survival compared with that reported previously (Guy et al., 2007), this is likely due to the use of a mixed C57BL6/CBA F2 genetic background in the current study, rather than the presence of elevated MeCP2 levels in these animals. Given the similarity between the phenotypes of Stop/y and Mecp2-null mice, we conclude that the ∼25–100-fold reduction in MeCP2 abundance is approximately equivalent to the deletion of the Mecp2 gene. Activation (de-silencing) of the Mecp2Stop allele was achieved by tamoxifen injection of mice, leading to translocation of the Cre-ESR fusion protein into the nucleus and excision of the Stop cassette. Southern blot analysis of 61 treated Stop/y,Cre mice revealed the recombination frequency in brain to be 69.8 ± 1.3% (range 52–83%; Fig. 1B). We also tested levels of MeCP2 protein following tamoxifen treatment by quantitative immunoblotting and found that treated Stop/y,Cre mice showed substantially increased levels of MeCP2 (Fig. 1C).
Silencing and rescue of MeCP2 expression in Mecp2Stop/y,Cre mice. (A) Quantitative western blots showing brain MeCP2 expression in wild-type (WT) and Stop/y males. Western blotting of whole brain extracts from wild-type and Stop/y littermates was used to quantify the amount of MeCP2 produced by the Stop allele. The amount of MeCP2 (boxed) was normalized to a non-specific cross-reacting band (asterisk) as a loading control. MeCP2 was measured for four Stop/y animals of different strain backgrounds, ages and aggregate symptom scores. (B) Southern blot showing recombination of the Stop/y allele (5.1 kb) to delete the Stop cassette (open triangle, 4.3 kb) after tamoxifen (Tx) treatment. All animals received the same tamoxifen-treatment regimen apart from #, which died soon after treatment started. (C) Representative western blot showing levels of MeCP2 protein in brains of wild-type, Stop/y and two tamoxifen-treated Stop/y;CreESRT animals. Recombination levels and the amount of protein relative to wild-type are shown. (D) Time plot showing phenotypic scores (see ‘Materials and methods’ section) for wild-type (open circle), Stop/y (black filled circles) and Stop/y,Cre mice (grey filled circles). Note the rapid symptom progression followed by a sustained improvement in symptom score following tamoxifen in the Stop/y,Cre cohort. (E) Recombination levels in brains of Stop/y,Cre mice showing relationship between higher recombination efficiency and milder symptom score at end of study.
To recapitulate previous studies, we utilized male mice that were hemizygous for the Mecp2Stop allele. Although a backcrossed C57BL6 background was used in our previous study (Guy et al., 2007), the poor breeding performance of these mice made it necessary to use an outbred genetic background for the aspects of this study requiring large cohorts of animals (breathing and behavioural analysis). Consistent with earlier data, however, these mice developed a range of overt signs including hypoactivity, irregular breathing, gait disturbances and hind limb clasping from around post-natal week 4–8. They also showed greatly reduced survival over the 16-week experiment. Reactivation of the Mecp2 allele in the Stop/y; CreESR line following tamoxifen treatment led to a sustained reduction in symptom severity (Fig. 1D) and increased survival as reported previously (Guy et al., 2007). In contrast, the Stop/y cohort, which lacked Cre and was therefore unable to respond to tamoxifen, showed progressively increasing phenotypic severity leading to premature death. All scoring was performed blind to genotype and treatment. Posthoc analysis revealed a negative correlation between final phenotypic scores and the level of MeCP2 activation as measured by recombination levels in Stop/y;Cre mice (Fig. 1E, linear regression, R2= 0.23, slope ≠ 0, P < 0.005). This indicates a causal relationship between the degree of symptom improvement and the number of cells expressing MeCP2 post-treatment.
Restoration of MeCP2 reverses structural deficits in cortical neurons
Severe motor impairments are a key feature of Rett syndrome (Nomura and Segawa, 1992) and are also seen in mice lacking MeCP2 (Chen et al., 2001; Guy et al., 2001, 2007; Luikenhuis et al., 2004). Corresponding structural abnormalities have also been reported in motor cortex of patients with Rett syndrome and Mecp2-null mice, including a thinning of the cortical layers and a reduction in neuronal size and complexity (Armstrong et al., 1995, 1998; Kishi and Macklis, 2004; Belichenko et al., 2009a,b). We wanted to determine whether gross phenotypic improvements seen previously upon reactivation of Mecp2 in mice (Guy et al., 2007) are accompanied by morphological changes within the adult nervous system. We focused our investigations on the primary motor cortex. Male Stop/y mice and wild-type littermate controls were sampled for morphometric analysis at 3 months of age, at which time the mutant mice displayed overt Rett-like signs (gross phenotype score = 4.3 ± 0.6). At the same time, an age-matched cohort of mice, including littermates of the Stop/y mice, which also carried the Cre transgene (Stop/y,Cre, mean symptom score = 4.3 ± 0.3), were given tamoxifen to instigate Mecp2 gene activation (de-silencing). These mice together with tamoxifen treated wild-type controls were then sampled for morphological analyses at 8–10 weeks following tamoxifen treatment. By this time the mean symptom score had reduced to 1.8 ± 0.3 in the Stop/y,Cre cohort. Unreactivated hemizygous Stop/y mice did not survive to this time point and were therefore unavailable as a matched control group.
Brains were Golgi stained and corresponding sections from each mouse (n = 16, four per group) assessed for a range of gross measures including neocortical thickness and thickness of the underlying corpus callosum (Fig. 2A and B). A random sample of layer 2/3 pyramidal cells (n = 210) was reconstructed by camera lucida to assess a range of cellular parameters, including soma size and various dendritic measures (Fig. 2C–E). Untreated Stop/y,Cre mice displayed significantly reduced thickness of motor cortex (83 ± 2.6% of control) and underlying white matter tract (83 ± 1.4% of control). At the cellular level, layer 2/3 pyramidal cells showed a consistent reduction in soma size (83 ± 2.7% of control), dendritic complexity and dendritic length, consistent with previous reports (Armstrong et al., 1995; Kishi and Macklis, 2004) (Fig. 2C–E). To quantify synaptic measures, secondary oblique dendrites in hippocampal area CA1 were assessed to reveal a significant reduction in spine density (78 ± 2.7% of control; n = 51–65 dendritic segments per group; Fig. 2E). Following tamoxifen treatment, all measured variables showed a trend towards wild-type levels. With the exception of cortical thickness, all parameters were not significantly different from their respective age-matched, wild-type controls (Fig. 2E; t-test, all P-values > 0.05) at 8–10 weeks post-tamoxifen. Further analysis confirmed a significant interaction between genotype and treatment for motor cortex soma size, dendritic length and hippocampal spine density (ANOVA, comparison of untreated Stop/y, treated Stop/y,Cre and corresponding wild-type mice, P < 0.05); Tukey’s posthoc comparison showing a significant treatment effect (all P-values < 0.05). While overall dendritic complexity showed a significant genotype difference between wild-type and both untreated and treated Stop/y,Cre mice (ANOVA, P < 0.05), neurons from untreated Stop/y mice showed significantly reduced values of dendritic complexity across 6 of 11 measured Sholl radii, whereas the post-treatment cohort differed from wild-type at only 2 of the 11 Sholl radii. These data provide evidence that restoration of Mecp2 to ∼70% of cells leads to the normalization of morphological changes caused by earlier deficiency of Mecp2.
Quantitative assessment of neuronal morphology in primary motor cortex following Mecp2 reactivation. (A) Golgi labelled brain sections from wild-type (Wt) and Stop/y,Cre mice were sampled for gross measures of cortical thickness (arrows) and corpus callosum (arrowheads) as well as layer 2/3 pyramidal cell morphology within primary motor cortex (hatched area). Analysis revealed reduced cortical thickness (B, representative micrographs) and reduced soma diameter (C) in Stop/y,Cre untreated mice. (D) Quantitative assessment of reconstructed cells (representative examples shown) by Sholl analysis (n = 50–60 cells/four animals per group, total 210 cells) revealed reduced dendritic branching complexity in Stop/y,Cre mice compared with wild-type littermate controls at Sholl radii 20–140 µm from soma. At 8–10 weeks following tamoxifen treatment, overall branching complexity was still reduced (P < 0.05, ANOVA followed by Tukey A post hoc analysis) compared with wild-type but this difference was restricted to Sholl radii between 60–80 µm from soma. (E) Pooled data revealed a significant (t-test comparison with age-matched wild-type, *P < 0.05) reduction in all parameters measured (cortical thickness, total dendritic length, length of basal dendritic tree, soma diameter and corpus callosum thickness) in Stop/y,Cre mice compared with wild-type littermates. A reduction was also observed in spine density (measured in primary oblique dendrites of hippocampal CA1 pyramidal cells as shown in insert; scale = 10 μm). Analysis of tamoxifen treated (rescued) mice revealed no significant difference from their appropriate littermate controls with the exception of cortical thickness, which remained significantly reduced compared with age-matched controls.
Normalization of respiratory measures upon Mecp2 reactivation
In addition to severe motor deficits, patients with Rett syndrome and Mecp2-deficient mice display a pronounced respiratory phenotype including apnoeas and irregular breathing patterns (Katz et al., 2009). We therefore tested the propensity for respiratory phenotype reversal upon reactivation of Mecp2 in adult mice by recording breathing patterns before and after tamoxifen treatment. In Stop/y,Cre mice, respiratory patterns varied within and between recordings, this variability was characterized by periods of hyperpnoea-like breathing (increased frequency) followed by periods of slow breathing due to prolonged expirations (Fig. 3A and C). Despite this, there was no significant difference in average respiratory frequency per se between Stop/y,Cre mice [310 ± 76 breaths per minute (bpm), n = 8] and wild-type littermate controls (305 ± 60 bpm, n = 11, P > 0.05; Fig. 3D) prior to tamoxifen treatment. In contrast, the coefficient of variation of respiratory frequency (CV%) was significantly higher in Stop/y,Cre mice (32 ± 17%, n = 8) when compared with wild-type littermate controls (16.8 ± 8.2%, n = 11, P < 0.05; Fig. 3E). Following tamoxifen treatment the breathing pattern in Stop/y,Cre mice became more regular with fewer periods of alternating fast and slow breathing. Indeed, there remained no significant difference in respiratory frequency between genotypes (Stop/y,Cre = 283 ± 65 bpm, n = 8 versus wild-type littermates = 286 ± 71 bpm, n = 11, P > 0.05) whereas the frequency variability reverted to wild-type levels in treated Stop/y,Cre mice (post-tamoxifen Stop/y,Cre CV% = 20 ± 11%, n = 8 versus post-tamoxifen wild-type littermates = 17 ± 9%, n = 11, P > 0.05) with posthoc tests indicating a significant improvement in frequency variability from pre- to post-treatment in Stop/y,Cre mice (P < 0.05).
Improved respiratory pattern following delayed activation of Mecp2. (A) Representative plethysmographic traces of wild-type (Wt) and Stop/y,Cre mice before (open symbols) and 5 weeks following tamoxifen treatment (filled symbols). Pre-tamoxifen treatment, the respiratory trace from a Stop/y,Cre mouse is characterized by periods of fast to normal frequency breathing interspersed with periods of slow breathing due to prolonged expirations. Post-tamoxifen treatment, the respiratory trace from the Stop/y,Cre mouse is similar to wild-type. Insert (i) is an illustration of the sigh-like breath indicated by the dashed lines in the Stop/y,Cre breathing trace. Insert (ii) is an example of a typical sigh, large amplitude breath followed by a prolonged expiratory pause. These sigh-like breaths were highly prevalent in Stop/y,Cre respiratory traces. Plotting the respiratory traces as Poincare plots (B, wild-type; C, Stop/y,Cre) shows an increased scatter, thus increased variability of breathing pattern, in Stop/y,Cre pre-tamoxifen treatment (open symbols) when compared with post-tamoxifen Stop/y,Cre and with wild-type. Overall, there was no significant difference in average baseline (i.e. apnoea-free segments) respiratory frequency (D) between groups (wild-type, n = 11; Stop/y,Cre n = 8); however the variability in respiratory frequency (E) was significantly increased in Stop/y,Cre mice pre-tamoxifen treatment when compared with post-tamoxifen treatment and wild-type. Pre-tamoxifen treatment, Stop/y,Cre mice exhibited an increased number of sigh-like bpm [F, A(i) and A(ii)], which was significantly reduced post-tamoxifen treatment (*P < 0.05).
We noted that Stop/y,Cre mice displayed an increased occurrence of sigh-like breaths [Fig. 3A(i), A(ii) and F]. More specifically these were large amplitude inspirations followed by a typical post-sigh expiratory pause, or large amplitude inspirations followed rapidly by a second smaller breath during the expiratory phase with no subsequent post-sigh expiratory pause. The occurrence of sigh-like breaths was significantly increased in Stop/y,Cre mice (3.2 ± 0.7 sighs per min, n = 8) compared with wild-type littermate controls (1.0 ± 0.1 sighs per min, n = 11). Post-tamoxifen, the occurrence of sighs decreased in Stop/y,Cre mice (1.2 ± 0.3 sighs per min, n = 8) similar to that seen in wild-type (0.9 ± 0.2 sighs per min, n = 11), again showing a significant treatment effect in Stop/y,Cre mice (P < 0.05). Our findings provide unequivocal quantitative evidence for functional improvement in specific breathing phenotypes following delayed activation of Mecp2.
Improvement in sensory-motor tasks after gene rescue
We next focused on the reversibility of sensory-motor skills. Overt neurological symptoms were quantified in different cohorts using a battery of sensorimotor tests. Tests were first conducted at a time when disease symptoms in Stop/y,Cre mice appeared mild–moderate (4–6 weeks of age). The Mecp2 gene was then activated and animals were retested 5 weeks later. Sensory-motor abilities were assessed on round and rectangular balance beams (Fig. 4A). Data pooled for beam size clearly revealed deficient performance compared with wild-type in Stop/y,Cre mice prior to treatment [Fig. 4A(i)]. Notably, MeCP2-deficient mice found smaller diameter beams difficult (interaction between beam size and genotype: P < 0.05). Upon treatment, Stop/y,Cre mice improved on all beam sizes (P < 0.05; posthoc Bonferroni: all P < 0.05) and no longer differed from wild-type controls at the large diameter beams (28 mm), indicating motor improvement after tamoxifen treatment. Stop/y,Cre animals still found the smaller beam sizes very challenging [Fig. 4A(ii)]. Wild-type mice also improved their performance after treatment (P < 0.05). Thus, Stop/y,Cre mice benefited considerably more from the treatment than controls and although sensory-motor skill is fully restored for simpler/wider beams, it is not fully rescued to wild-type levels.
Improvement in balance and motor function following activation of Mecp2. [A(i)] Both Stop (n = 24) and Stop/y,Cre (n = 17) mice displayed similar impairment in balance beam performance compared with wild-type pretreatment at all beam widths tested (5–28 mm round and rectangular beams combined). [A(ii)] Following tamoxifen treatment, Stop/y,Cre (n = 17) mice improved performance when tested on the large (28 mm) beams, but remained significantly impaired relative to wild-type in the narrower beams. Note that impairment became more pronounced as the task was made more challenging with narrower beams. [B(i)] Grip strength at pretreatment showed significant impairment in Stop/y,Cre cohort; [B(ii)] there was no difference between genotypes 6 weeks after tamoxifen treatment. In contrast, swim speed recorded in a continuous swim task was lower in Stop/y,Cre mice pre- and post-tamoxifen treatment [C(i) and (ii)]. Performance on the rotarod was significantly reduced for maximum attained rotation speed [D(i)] and for motor learning [E(i)] in Stop/y,Cre mice pretreatment. This phenotype fully recovered following tamoxifen administration [D(ii) and E(ii)]. Not affected by treatment were parameters of gait as determined by CatWalk. There was a shorter stride length for all paws [F(i) and (ii)] and greater paw distance between the hind, but not front legs [G(i) and (ii)], both pre- and post-treatment, respectively. Means ± SEM. Asterisks indicate P < 0.05 relative to wild-type.
Loss of muscle strength, possibly related to degeneration of spinal cord motor neurons (Oldfors et al., 1988) occurs early in the Rett syndrome disease process. This parameter was assessed with a grip-strength meter prior to and following gene reactivation (Fig. 4B) in wild-type and Stop/y,Cre mice. The initial grip-strength deficit (P < 0.05) in Stop/y,Cre mice was fully recovered after tamoxifen injections. Indeed, no phenotype was detectable 5 weeks post-treatment [Fig. 4B(ii)] [interaction of genotype and test-phase (before and after treatment) as factors, P < 0.05; for post hoc, see asterisks in Fig. 4B]. This was due in part to a reduction of grip strength in wild-type (P < 0.05) but also to a reliable improvement in grip strength in Stop/y,Cre mice post-reactivation (P < 0.05). Three further measures pertaining to motor movement and muscle strength were undertaken. Firstly, mice were tested on the rotating rod so that they were compelled to progress in order to avoid falling off. The latency time until descent was initially recorded for all trials, and then converted into rotations per min (rpm) sustained during each trial/session (Fig. 4D). While genotypes differed significantly during pretreatment for both compound measures [Fig. 4D(i)] (overall two-way ANOVA, main effect of genotype P < 0.05, post hoc P < 0.05; n.s. for post-treatment results), tamoxifen exposure completely rescued this phenotype and there was no difference between groups after treatment [Fig. 4D(ii)]. This was due to an improvement of Stop/y,Cre mice after treatment (P < 0.05) while wild-type did not change. Similar results were obtained for motor learning indexed as improvement from Trial 1 to Trial 8. Although both genotypes presented with motor learning (wild-type: P < 0.05; Stop/y,Cre: P < 0.05), performance was lower for Stop/y,Cre mice (Fig. 4E) pre- but not post-treatment suggesting complete rescue of this phenotype. As a second paradigm for enforced movement, we determined swim speed recorded in a water maze during a 30 s swim period (Fig. 4C). In line with the rotarod results, Stop/y,Cre mice swam slower than wild-type (P < 0.05 for genotype, no interaction with test phase). The pretreatment difference [Fig. 4C(i), P < 0.05] persisted after Mecp2 gene activation [Fig. 4C(ii); P < 0.05], but there was a significant improvement in this marker from pre- to post-treatment in Stop/y,Cre mice (P < 0.05), but no change in wild-type. These findings add support to the notion that late restoration of MeCP2 leads to recovery of movement-related disabilities. To further test aspects of motor function we conducted a gait analysis. Front/hind paw stride length (Fig. 4F) and paw width (Fig. 4G) measures were obtained using the CatWalk (see ‘Materials and methods’ section). Both markers were reliably different between genotypes [Fig. 4F(i) and 4G(i)], suggesting that a wider hind paw width leads to smaller stride length in Stop/y,Cre mice. Interestingly, these phenotypes were not recovered after tamoxifen treatment [Fig. 4F(ii) and G(ii)]. It thus appears that neuromuscular defects affecting gait may be less reversible by Mecp2 gene activation than other aspects of the phenotype or take longer to recover.
Structural plasticity in the Rett syndrome brain
Neurobiological orthodoxy holds that structural abnormalities arising from abnormal brain development result in a range of neurological and psychiatric symptoms that are essentially irreversible in adults. Hence Rett syndrome is routinely classified as a neurodevelopmental disorder on the assumption that MeCP2-deficiency during development is at the root of this condition. Several phenotypes such as disturbances in calcium homeostasis in cultured neurons (Mironov et al., 2009) are evident at early developmental time points in Mecp2-null mice and early neuronal defects are also detected in induced pluripotent stem cells derived from patients with Rett syndrome (Marchetto et al., 2010; Cheung et al., 2011). Moreover, various clinical studies report discrete alterations in the pre-symptomatic phase (Charman et al., 2002) while early effects have also been seen in Mecp2 mutant mice (Picker et al., 2006; Santos et al., 2007; De Filippis et al., 2010). Against this conventional classification however, functional studies in a range of animal models, including our previous work on MeCP2-deficient mice (Guy et al., 2007), demonstrate that reversing or compensating for some of the underlying molecular deficits in adult mice can result in substantial improvements in function (Ehninger et al., 2008). In particular, almost complete reversal of Rett syndrome-like symptoms was observed in females heterozygous for a Mecp2-STOP allele even though the animals were >6 months old and therefore long past any known developmental event. The implication of these findings is that development in the absence of MeCP2 does not irreversibly compromise all subsequent brain function. In short, they suggest that Rett syndrome may defy simple classification as a neurodevelopmental disorder. A potential caveat to this revisionist view could be that reversal applies only to superficial features of the Rett syndrome-like phenotype, leaving fundamental aspects of neurological function in the original defective state. In our earlier study, reversal of impaired survival, obesity and hippocampal long-term potentiation were assessed quantitatively, but other aspects of phenotype, including gait, breathing, mobility, tremor and general condition were assayed using a ‘light touch’ observational protocol that could be applied on a weekly basis over many months (Guy et al., 2007). The purpose of the present study was to assess the reversibility of a range of phenotypic traits in a more robust and quantitative manner.
Although several ‘neurodevelopmental disorders’ show evidence of a degree of reversal, there have been few studies of the extent to which defects in brain morphology can be structurally repaired in vivo. Morphological abnormalities including altered neuronal packing density, altered neuronal size and dendritic complexity have been reported both in human Rett syndrome (Armstrong et al., 1995, 1998; Belichenko et al., 1997; Armstrong, 2005) and MeCP2-deficient animal models (Kishi and Macklis, 2004; Belichenko et al., 2008, 2009a, b; Jentarra et al., 2010). At a gross level the Stop/y mouse brain appears relatively normal in terms of lamination and architecture, but at a cellular level we confirmed reduced neuronal size and dendritic length and complexity within the primary motor cortex. All of these defects were significantly improved following Mecp2 activation, approaching or reaching wild-type levels. We conclude that MeCP2-deficient neurons exhibit considerable structural plasticity even in a nervous system that is fully adult. However, the lack of an available comparison with untreated Stop/y,Cre mice (which do not survive), somewhat hinders a straightforward ‘treatment–effect’ interpretation. These findings nevertheless extend previous studies showing that deficits in dendritic, synaptic and axonal morphologies of MeCP2-deficient neurons are reversible in cultured systems following reintroduction of MeCP2 (Rastegar et al., 2009) or by pharmacological interventions targeting aberrant signalling processes (Larimore et al., 2009; Tropea et al., 2009) or by targeting astrocyte function (Lioy et al., 2011).
A prominent feature of many patients with Rett syndrome is microcephaly. Unlike other neuronal measures, which showed a marked reversal of morphological impairment, the gross measure of neuropil (cortical thickness) was not reversed to a statistically significant extent. Thus structural plasticity at the cellular level may not be mirrored in the surrounding skull. Indeed, we know from previous work that very rapid activation of MeCP2 (over days) is detrimental while a more gradual reactivation regime (over weeks) avoids this lethality (Guy et al., 2007). The possibility that abrupt remodelling of the nervous system within the confines of a microencephalitic skull is deleteious and remains to be investigated.
Delayed activation of MeCP2 stabilizes respiratory function
Breathing abnormalities are a prominent feature of Rett syndrome, including irregular respiratory patterns during wakefulness, breath holding, sighs and apnoeas (Julu et al., 2001). Whole body plethysmography confirmed the presence of an overt breathing phenotype in the Stop/y,Cre mice, including increased variability of breathing pattern and the increased occurrence of abnormal breaths (Fig. 3). These findings are consistent with similar measures conducted in other Mecp2-mutant mouse lines (Viemari et al., 2005; Ogier et al., 2007; Roux et al., 2007; Tropea et al., 2009; Abdala et al., 2010; Pratte et al., 2011). We show here that late activation of the Mecp2 gene generates a robust improvement in breathing patterns in the mice with Rett syndrome, including a near complete reversal of breathing pattern dysrhythmias and reduced incidence of abnormal sigh-like breaths. The brainstem pathology underlying the Rett syndrome respiratory phenotype is not fully understood but has been the subject of intensive research particularly testing putative pharmacological therapies. Previous studies have shown improvement of respiratory rhythm in Mecp2-null male mice by application of desipramine to target the noradrenergic system (Roux et al., 2007) or in MeCP2-deficient female mice by combining a GABA reuptake blocker with a 5HT1a agonist (Abdala et al., 2010). Taken together with the results of this study and the recent report by Lioy and colleagues (2011) focusing on astrocyte function, the respiratory phenotype may be a therapeutically tractable feature of Rett syndrome.
Sensory-motor dysfunction is rescued by late Mecp2 gene activation
A number of studies have previously characterized changes in performance in similar tasks in a number of MeCP2-mutant lines (Stearns et al., 2007; Kondo et al., 2008; Pratte et al., 2011) and our findings in the Stop/y hemizygous mouse were consistent with deficits seen in Mecp2-null studies. Following reactivation of Mecp2 there was evidence for modest but significant improvement across a wide range of motor and locomotor tasks. We did not attempt to directly relate observed morphological changes in motor cortex with functional effects that presumably involve a range of brain structures/circuits. It is clear however, that late reactivation of the Mecp2 gene caused a quantitative improvement in several motor functions including coordination and balance (rotarod and balance beam). Also muscular strength was restored to almost wild-type levels. Swim speed increased after Mecp2 gene activation, but remained significantly lower than wild-type. Least reversible were defects in gait, which persisted at significant levels in otherwise ‘rescued’ animals. Failure to fully reverse symptoms could be taken as evidence that some defects are not rectified by restoration of MeCP2. It is also possible that some phenotypes may show a more protracted or delayed rescue than others. There are, however, two confounding issues that qualify this interpretation. Firstly, activation affects 70% of brain cells on average, leaving 30% highly deficient in MeCP2. We do not know that all phenotypes can be rectified by such a mosaic genetic rescue. Secondly, due to limited survival of Stop/y animals, unreversed mice were not available for testing 5 weeks after tamoxifen treatment. This means that mutant mice before and after gene reactivation were compared with wild-type littermates. The results were unambiguous in cases where the defect was fully reversed to the wild-type level, but the defect that persists, abnormal gait, was less easy to interpret. This difficulty arises because Stop/y,Cre animals were relatively mildly affected when the experiment began. Therefore, a parameter that appears to remain unchanged relative to wild-type after Mecp2 activation is being compared with that of a weakly symptomatic animal and does not take into account the phenotypic decline that follows. Persistence of a phenotypic feature in the Mecp2-reactivated animals may therefore represent significant stabilization of a sign that would almost certainly have become progressively more severe during the lifetime of the animal. Indeed, a recent study in which deletion of Mecp2 in the adult mouse recapitulates the phenotype of germ line knockout of Mecp2 would support the line that MeCP2 has a necessary role beyond development and throughout adult life (McGraw et al., 2011). In a clinical neurology context, this report coupled with the current findings suggest that therapeutic amelioration of features associated with MeCP2 insufficiency may be clinically achievable, but with the possible exception of gene replacement therapy, any potential treatment may need to be lifelong rather than transient therapeutic intervention delivered during a critical or sensitive periods of development.
In summary, we have measured reversibility of fundamental aspects of the Stop/y phenotype and find that the great majority become significantly less severe when MeCP2 is restored in ∼70% of cells. Importantly, neuronal morphology is rectified, indicating significant plasticity in the adult mouse. Our findings suggest that a ∼25-fold reduction in the level of MeCP2 during brain development has no lasting consequences, as late administration of MeCP2 can reverse the observed defects. It has previously been suggested that MeCP2 is not required for brain development, but plays a role in maintaining neurological function once development is complete (Guy et al., 2001, 2007; Kishi and Macklis, 2004). The current findings sustain this and they highlight the need for a more complete description of the role played by MeCP2 in brain cell homeostasis.
Medical Research Council (G0800401); Wellcome Trust; Scottish Rett Syndrome Association and Rett Syndrome Research Trust.