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Mice carrying bacterial artificial chromosome (BAC) transgenes have become important tools for neuroscientists, providing a powerful means of dissecting complex neural circuits in the brain. Recently, it was reported that one popular line of these mice – mice possessing a BAC transgene with a D2 dopamine receptor (Drd2) promoter construct coupled to an enhanced green fluorescent protein (eGFP) reporter – had abnormal striatal gene expression, physiology and motor behavior. Unlike most of the work using BAC mice, this interesting study relied upon mice backcrossed on the outbred Swiss Webster strain that were homozygous for the Drd2-eGFP BAC transgene.The experiments reported here were conducted to determine whether mouse strain or zygosity was a factor in the reported abnormalities. As reported, SW mice were very sensitive to transgene expression. However, in more commonly used inbred strains of mice (C57BL/6, FVB/N) that were hemizygous for the transgene, the Drd2-eGFP BAC transgene did not alter striatal gene expression, physiology or motor behavior. Thus, the use of inbred strains of mice which are hemizygous for the Drd2 BAC transgene provide a reliable tool for studying basal ganglia function.
Mice carrying engineered BAC transgenes have become an important tool for neuroscience research (Gong et al., 2003; Gong et al., 2010). By inserting an expression cassette that contains the regulatory elements of a particular gene into a BAC vector, it has been possible to drive the expression of a genetically encoded fluorescent reporter (e.g. eGFP or tdTomato) or Cre recombinase in specific neuronal populations. Using this technology, the GENSAT (Gene Expression Nervous System Atlas, NIH-NINDS) project has generated over 1000 mouse lines with targeted cellular expression of GFP or Cre (Heintz, 2001; Gong et al., 2003; Siegert et al., 2009).
These mice have been a major resource to the neuroscience community and have enabled a wide range of previously unaddressable questions to be answered. For example, dopamine (DA) receptor BAC transgenic mice have been instrumental in allowing neurophysiologists and neuroanatomists to interrogate the two principal populations of spiny projection neurons (SPNs) in the striatum. Although these two populations play very different functional roles in the basal ganglia (Albin et al., 1989; DeLong, 1990; Albin et al., 1995), they are intermingled and have similar somatodendritic morphology making them impossible to reliably distinguish visually. One distinguishing feature of these two populations is their expression of DA receptors. SPNs that project primarily to the substantia nigra, so-called direct pathway SPNs (dSPNs), express the Drd1a (DA D1 receptor), whereas SPNs that project to the globus pallidus, so-called indirect pathway SPNs (iSPNs), express the Drd2 (DA D2 receptor). BAC transgenic mice in which GFP expression is driven either by a Drd1a or a Drd2regulatory elements construct allow the visual identification of these SPNs in either fresh or fixed tissue, providing an enormous experimental advantage.
The utility of these mice depends upon the assumption that the transgene itself has little or no effect on phenotype. However, there are situations in which this assumption could be invalid. For example, the BAC construct invariably has sequences of unknown or poorly characterized function; if expressed, these sequences could alter cellular phenotype. In addition, chromosomal integration of the BAC construct could have effects on native gene expression that are independent of the transgene itself. Both of these effects could be sensitive to transgene copy number. As a consequence, BAC transgenic mice should be used with circumspection.
Recently, Kramer and colleagues (Kramer et al., 2011) reported that Swiss Webster (SW) mice that were homozygous for the Drd2-eGFP BAC transgene had an altered phenotype. In particular, they found significant abnormalities in the release of DA and in the response to cocaine administration. Given the growing use of these mice, we felt it was important to pursue these interesting findings. Although we were able to reproduce their observations in hemizygous SW mice, we did not find detectable changes in striatal gene expression, striatal physiology or motor behavior in hemizygous FVB/N or C57BL/6 Drd2-eGFP transgenic mice.
All experiments detailed are in accord with the Northwestern University Animal Care and Use Committee, and are in compliance with the NIH Guide to the Care and Use of Laboratory animals. Unless otherwise noted, all experiments were conducted with Drd2-eGFP BAC transgenic mice on an FVB/NJ (inbred; Jackson Laboratory), C57BL/6J (inbred; Jackson Laboratory), and Swiss Webster (outbred; Taconic Farms) backgrounds. The original founder animals were a gift from Drs. N. Heintz and P. Greengard (The Rockefeller University). They were generated by injection of a modified BAC (containing eGFP under the regulatory elements of the Drd2 gene) into pronuclei of FVB/N fertilized oocytes. Subsequently, zygotes were injected into pseudo-pregnant female Swiss Webster (an outbred strain from Taconic) (Gong et al., 2010). All Drd2-eGFP BAC transgenic mice in this study were back-crossed with wild-type inbred breeders for at least 7-9 generations to create hemizygote FVB/N and C57BL/6 animals. The FVB/N line was outcrossed with the Swiss Webster animals for up to two generations for this study. All animals included in this study were males (unless otherwise indicated) between 3-5 weeks of age and housed and bred in the same environment. Transgene copy number was confirmed with tail biopsy using real-time quantitative PCR (with primers direct against the chloramphenicol-resistance gene of the BAC vector and Gapdh). Comparison was made using □□CT method (see below) with known standards.
Unilateral lesion of the nigrostriatal system was produced by 6-hydroxydopamine (6-OHDA) injection into the medial forebrain bundle (MFB). In brief, mice at postnatal day 28-32 were anesthetized with a mixture of ketamine (50 mg/kg i.p.) and xylazine (4.5 mg/kg i.p.). After immobilization on a stereotaxic frame (David Kopf Instruments) with a Cunningham adaptor (Harvard Apparatus), a hole was drilled (~1 mm diameter) at 0.7 mm posterior and 1.1 mm lateral to bregma for injection into the MFB (0.7 AP = anterior-posterior, 1.1 ML = medial-lateral, 4.8 DV = dorsal-ventral). 1 μL of 6-OHDA HCl (Sigma Chemical Co.) was dissolved at a concentration of 7.5 μg/μl saline with 0.02% ascorbate and injected using a calibrated glass micropipette (Drumond Scientific Co.), at a rate of 0.02 μl/min and at a depth of 4.8 mm from the surface of the skull. The micropipette was left in situ for another 30 minutes after the injection to maximize tissue retention of 6-OHDA and decrease capillary spread upon pipette withdrawal. Electrophysiological experiments were performed 3-4 wks later.
Eticlopride HCl (1 mg/kg; Tocris Bioscience) was dissolved in sterile PBS and stored at 4°C. Homozygous Drd2-eGFP FVB/N mice (3-4 week) were injected intraperitoneally (i.p.) once daily for 14 days. Animals were killed for recording 24 hours after the last injection to ensure the clearance of eticlopride and its metabolites from the brain.
An open field arena (56 × 56 cm) was used for measuring non-reinforced ambulatory behavior of animals (4-5 weeks of age). Each arena was cleaned with disinfectant prior to the testing of each subject. Behavioral assessment of subjects were performed between 3:00-6:00 pm with the ambient light set at 35 lux. An individual mouse was placed in the center of the arena and its ambulation and exploratory activity was recorded by a CCD camera connected to a personal computer. Video tracking of animals was performed for 20 minutes using LimeLight2 (Coulbourn Instruments) at rate of 3.75 frames per second. The arena contained a 10×10 grid block on the bottom surface to allow off-line analysis of the animals’ movement in specific regions of the arena. In each session, the total distance traveled as well as the percentage of time/distance within different parts of the arena were recorded. Behavioral assays were performed at the Northwestern University Behavioral Phenotyping Core Facility.
Western blotting procedures were similar to that previously described (Chan et al., 2011). In brief, membrane protein fractions were prepared by lysis of tissue in buffer containing 10 mM HEPES, pH 7.4, and 320 mM sucrose, followed by brief centrifugation to remove nuclei and insoluble material. After centrifugation at 16,000x g, the pellet was resuspended by gentle rocking at 4 °C in TEEN-Tx (0.1 M Tris, 1 mM EDTA, 1 mM EGTA, and 1% Triton X-100). Protein extracts were resolved by SDS-PAGE, and transferred to polyvinylidene difluoride membranes. Western blotting was performed using Drd2 primary antibody at a concentration of 1μg/ml (a gift from Ryuichi Shigemoto, National Institute for Physiological Sciences, Okazaki, Japan).
Quantitative polymerase chain reaction (qPCR) was used to determine the abundance of transcripts of interest with procedures similar to that described previously (Chan et al., 2011). In brief, striata were microdissected in ice-cold aCSF from a series of 300 μm tissue slices. Total RNA was isolated using RNeasy micro kit (Qiagen). cDNA was synthesized using qScript cDNA Supermix (Quanta Biosciences). Real-time PCR was performed using Fast SYBR Mastermix (Applied Biosystems) on a StepOnePlus thermocycler (Applied Biosystems). The thermal cycling conditions comprised of an initial denaturing step at 95°C for 20 s, and 40 cycles at 95°C for 3 s, 60°C for 30 s. The PCR cycle threshold (Ct) values were measured within the exponential phase of the PCR reaction using StepOnePlus software version 2.1 (Applied Biosystems). A correction was performed using a passive reference dye (Rox) present in the PCR master mix. Reactions with any evidence of nonspecificity (i.e. low melting temperatures or multiple peaks in melting point analysis) were excluded from the analysis. A relative quantification method (i.e. □□CT method) was used to quantify differences in gene expression level (Schmittgen and Livak, 2008). To increase accuracy of the gene expression analysis, a panel of reference genes (Atp5b, Cyc1, Eef1e1, Gapdh, Gusb, H2afz, Hmbs, Sdha, Uchl1) were included in order to establish an ensemble reference — weighted Cts based on the stability of each reference gene were calculated from established algorithms (Vandesompele et al., 2002; Andersen et al., 2004; Pfaffl et al., 2004; Silver et al., 2006), as described in equations 1-3.
R is a relative value that incorporates the rank values of all the reference genes for a particular algorithm. αRG represents the average R value calculated using 4 different algorithms. CtRG is the Ct value of a reference gene for an individual sample. Experiments for each gene of interest were run in triplicates. Desalted primers were custom synthesized (Invitrogen) and intron-spanning whenever possible. No-template and no-reverse-transcriptase control assays produced negligible signals, suggesting that primer dimer formation and genomic DNA contamination effects were small. The mRNA levels in each subgroup of samples were characterized by their median values. Results were presented as fold difference relative to their respective wild-type controls. Data are presented as median fold difference and median experimental error (standard deviation) (Bookout et al., 2006). Statistical analysis (Mann-Whitney U test) was performed. Differences between the genotypes were judged significant at confidence levels of 95% (P<0.05).
Mice (males, 3-5 weeks old) were anesthetized with ketamine/xylazine and perfused transcardially with ice cold artificial cerebrospinal fluid (aCSF) containing in mM: 125 NaCl, 2.5 KCl, 1.25 NaH2PO4, 2.0 CaCl2, 1.0 MgCl2, 25 NaHCO3, and 12.5 glucose, bubbled continuously with carbogen (95% O2 and 5% CO2). The brains were rapidly removed, glued to the stage of a slicer (Leica), and immersed in ice-cold aCSF. Striatal slices were cut at a thickness of 240-275 μm and transferred to a holding chamber, where they were submerged in aCSF at 35°C for 30 minutes, and returned to room temperature before recording. SPNs within the dorsal striatum were identified by their somatic morphological characteristics under IR-DIC or Dodt-contrast optics. Somatic eGFP expression was verified using epifluorescence microscopy to confirm cell identity before breaking into whole-cell mode. Recordings were made at room temperature (20-22°C) with patch electrodes (1.5 mm outer diameter) fabricated from filamented, thick-wall borosilicate-glass (Sutter Instruments) pulled on a Flaming-Brown puller (Sutter) and fire polished immediately before use. Pipette resistance was typically ~3-5 MΩ. For current-clamp recordings, the internal solution consisted of (in mM): 135 KMeSO4, 5 KCl, 10 Na2-phosphocreatine, 5 EGTA, 0.5 CaCl2, 2 Mg-ATP, 0.5 Na3-GTP, 5 HEPES, adjusted to pH 7.25-7.30 with KOH, 300 mOsm. The liquid junction potential in recordings was ~7 mV and was not corrected for. For voltage-clamp experiments, pipettes were filled with a Cs+-based internal solution containing (in mM): 125 CsMeSO3, 5 TEA-Cl, 10 Na2-phosphocreatine, 5 HEPES, 0.25 EGTA, 2 Mg-ATP, 0.5 Na-GTP, 1 QX-314-Cl, adjusted to pH 7.25-7.30 with CsOH, 300 mOsm. Electrical stimulation (200-400 μs) was performed using parallel bipolar tungsten electrodes (Frederick Haer & Co) placed in the layer V-VI of the cortex. Somatic whole-cell patch-clamp recordings were obtained with an amplifier (Molecular Devices). The signal for voltage clamp recordings was filtered at 1 kHz and digitized at 10 kHz with a digitizer (Molecular Devices). For current-clamp recordings, the amplifier bridge circuit was adjusted to compensate for electrode resistance and subsequently monitored.
SPN in tissue slices (as described above) were loaded with Alexa Fluor 594 (50 micromolar) through the patch pipette. All experiments were performed at room temperature. Images were acquired with a 60X/1.00 NA water-immersion lens (Olympus). The two-photon excitation source was a Chameleon-Ultra2 tunable laser system (680 to 1080 nm) using titanium:sapphire gain medium with all-solid-state active components and a computer-optimized algorithm to ensure reproducible excitation wavelength, average power, and peak power (Coherent Laser Group). Optical signals were acquired using 810 nm excitation beam (80-MHz pulse repetition frequency and 250 fs pulse duration) to excite Alexa 594. The fluorescence emission was collected by external or non-descanned photomultiplier tubes (PMTs). The red fluorescence (580-640 nm) was collected by a multi-alkali-cathode (S-20) PMT. Measurements were taken in a sample plane along dendritic segments (>50 μm from the soma). On average, ~80 spines were counted per dendritic segments; up to 3 measurements were performed on each cell.
Curve fitting and data analyses were done with ClampFit 9 (Molecular Devices), Igor Pro 6.0 (Wavemetrics), MATLAB 7.12 (MathWorks), MiniAnalysis 6.0.3 (Synaptosoft), and Prism 5 (GraphPad). Box plots were used for graphic representation: the central line represents the median, the edges represent the interquartile ranges, and the whiskers represent the overall distribution. Asterisks indicate 95% confidence (p<0.05) unless otherwise noted. Normal distributions were not assumed regardless of sample size or variance. Pairwise comparisons for unrelated samples were performed using a Mann-Whitney U test with a threshold of p<0.05 for significance. Kruskal–Wallis one-way analysis of variance was performed for group comparisons with a threshold of p<0.05. Frequency-intensity (F-I) curves were analyzed with two-way repeated measures analysis of variance, with SPN type or treatment group and current injection as independent variables. Group main effect between SPN type or treatment group is reported. Significance was set as α = 0.05.
The expression cassette in the BAC vector used in creating the Drd2-eGFP line was constructed by the insertion of a polyadenylated reporter gene (i.e., eGFP) into the Drd2 locus immediately downstream of the ATG translation initiation codon. The removal of the Drd2 coding sequence downstream from the initiation codon rendered no functional Drd2 RNA or protein expression from the BAC vector. Surprisingly, the study by Kramer et al. (Kramer et al., 2011) found that there was overexpression of the Drd2 gene, in SW mice that were homozygous for the Drd2-eGFP transgene. To determine if zygosity was a factor in this effect, quantitative real-time PCR (qPCR) profiling for 21 transcripts was performed on striatal tissue derived from four different lines of mice of varying strain and zygosity for the Drd2-eGFP transgene (Fig. 1; Table 1). In hemizygous SW mice, there was a modest (~1.5 fold), but significant elevation in Drd2 mRNA (p<0.05, Mann-Whitney U Test). However, in hemizygous C57BL/6 and FVB/N mice there was no detectable change in Drd2 expression level (p>0.05, Mann-Whitney U Test). In homozygous FVB/N mice, on the other hand, Drd2 expression was significantly elevated (~2 fold) (p<0.05, Mann-Whitney U Test). This was not a consequence of amplification of the truncated Drd2 transgene in the BAC vector, as primers were directed against only the full-length Drd2 sequence. This analysis also found that in homozygous FVB/N mice there was a concomitant upregulation of Drd1a and Adora2a (adenosine A2a receptor) (Fig. 1) (p<0.05, Mann-Whitney U Test).
It has been suggested that Ttc12 is a ‘passenger’ gene in the Drd2-eGFP BAC construct that might alter cellular phenotype (Kramer et al., 2011). If this were true, zygosity should dictate Ttc12 RNA levels. Although the abundance of Ttc12 RNA was correlated with zygosity, its expression also varied with mouse strain (Fig. 1). At this point, we do not know if this has any causal effect on the phenotype of the striatum.
To determine whether the Drd2-eGFP transgene altered striatal physiology, whole-cell recordings were made from iSPNs and dSPNs in brain slices from three different strains of transgenic mice.
First, the intrinsic excitability of each population of SPNs was assessed by constructing plots of spike rate as a function of current injected through a somatic electrode; these plots are called frequency-intensity (F-I) curves. Several groups have reported that iSPNs are more excitable than dSPNs, as manifested by F-I curves that are shifted to the left along the current axis (Kreitzer and Malenka, 2007; Ade et al., 2008; Gertler et al., 2008). This dichotomy was preserved in hemizygous and homozygous Drd2-eGFP BAC FVB/N mice (Drd2 FVB/N hemi: iSPNs n=19, dSPNs n=12; Drd2 FVB/N homo: iSPNs n=14, dSPNs n=15; Group main effect, p<0.01, two-way repeated measures ANOVA) (Fig. 2A,B). However, in homozygous mice, the excitability of iSPNs neurons was significantly increased compared to iSPNs in hemizygous FVB/N mice. (Table 2, Group main effect, p<0.001, two-way repeated measures ANOVA) (Fig. 2B); in this figure, the F-I curve for the hemizygous mice is plotted as a dashed line for comparison. To determine if the dichotomy was an artifact of the Drd2-eGFP transgene, GFP-positive and negative SPNs were sampled from hemizygous Drd1a-GFP BAC transgenic FVB/N mice, which have no apparent adaptation in response to transgene expression (Ade et al., 2011). In these mice, GFP-negative neurons were assumed to be iSPNs, as shown by previous work (Gertler et al., 2008). The F-I curves of dSPNs and iSPNs in these mice were very similar to those in hemizygous Drd2-eGFP mice (Drd1a FVB/N hemi: iSPNs n=22, dSPNs n=22; Group main effect, p>0.05, two-way repeated measures ANOVA) (Fig. 2C, Table 2), arguing that the dichotomy was not an artifact and that, in hemizygous FVB/N mice, the transgene had no effect on intrinsic excitability.
To pursue the potential effects of mouse strain, hemizygous C57BL/6 and SW mice were also examined. In hemizygous C57BL/6 mice, the excitability of dSPNs and iSPNs was significantly different (Drd2 C57BL/6 hemi: iSPNs n=21, dSPNs n=16; Group main effect, p<0.001, two-way repeated measures ANOVA) – as found in hemizygous Drd2-eGFP FVB/N mice (Fig. 2D, Table 2). In contrast, there was not a significant difference between dSPNs and iSPNs in hemizygous Drd2-eGFP SW mice (SW hemi: iSPNs n=5, dSPNs n=7; Group main effect, p>0.05, two-way repeated measures ANOVA) (Fig. 2E, Table 2). This phenotypic difference was unlikely to have been a consequence of elevated Drd2 expression, however, as this should have increased the excitability of iSPNs and these cells were very similar in SW and FVB/N mice (Table 2, Group main effect, p>0.05, two-way repeated measures ANOVA) (cf., Fig. 2E,A). Rather, the similarity in SW SPNs was attributable to a relative shift in the excitability of dSPNs (see dotted red line for comparison), suggesting that strain differences, not the transgene, was responsible.
To provide an assay of network physiology to complement the assessment of intrinsic excitability, the synaptic connectivity between cortical pyramidal neurons and SPNs was examined. Both short- and long-term plasticity of this synapse is controlled by DA and potentially sensitive to alterations in Drd2 expression (Gerfen and Surmeier, 2011). Short-term excitability of this synapse was examined using a paired-pulse protocol (Zucker and Regehr, 2002; Branco and Staras, 2009). There were no detectable differences in the paired-pulse ratio of corticostriatal synapses on iSPNs, measured at 50 Hz (Fig. 3A), as a function of strain or zygosity of animals (FVB/N homo median = 1.070, n = 17; FVB/N hemi median = 1.325, n = 12; C57BL/6 hemi median = 1.465, n = 14; p>0.05, Kruskal-Wallis test). Similarly, there were no differences in the frequency (FVB/N homo median = 2.92 Hz, n = 11; FVB/N hemi median = 2.98 Hz, n = 7; C57BL/6 hemi median = 2.77 Hz, n = 8) or amplitude (FVB/N homo median = 11.73 pA, n = 11; FVB/N hemi median = 11.99 pA, n = 7; C57BL/6 hemi median = 11.63 pA, n = 8) of miniature excitatory synaptic currents (mEPSCs) in any of these lines (p>0.05, Kruskal-Wallis test) (Fig. 3B), arguing that the release probability at glutamatergic synapses, as well as their number, was unaltered by expression of the Drd2-eGFP transgene. In agreement with this inference,in iSPNs the density of dendritic spines – membrane specializations where glutamatergic synapses are formed – was not affected by strain or transgene zygosity (SW hemi median = 1.85 spine/μm, n = 8; FVB/N homo median = 1.78 spine/μm, n = 5; FVB/N hemi median = 1.64 spine/μm, n = 5) (p>0.05, Kruskal-Wallis test) (Fig. 3C).
The data from homozygous FVB/N suggests that an elevation of Drd2 signaling can decrease the intrinsic excitability of iSPNs. To test this hypothesis, homozygous FVB/N mice were subjected to two manipulations aimed at decreasing Drd2 activity. First, homozygous Drd2-eGFP mice were depleted of dopamine by the injection of the toxin 6-hydroxydopamine (6-OHDA) into the medial forebrain bundle; these lesions deprived the striatum of more than 90% of its dopaminergic innervation. Three to four weeks after this lesion, iSPNs were recorded in brain slices from these mice and unlesioned controls. As predicted, the F-I curves of iSPNs in dopamine-depleted mice were shifted to the right along the current axis (Naïve: n=35; 6-OHDA: iSPNs n=14; Group main effect, p<0.001, two-way repeated measures ANOVA) (Fig. 4A,B). To provide an alternative test, mice were administered the Drd2 antagonist eticlopride for 2 weeks. Again, iSPNs from treated mice were less excitable (naïve: n=35; eticlopide: n=16; Group main effect, p<0.001, two-way repeated measures ANOVA) and had F-I curves that were shifted toward higher currents (Fig. 4A, bottom, dashed line). Together, these data show that alterations in Drd2 signaling can influence the intrinsic excitability of iSPNs, suggesting that the elevated intrinsic excitability of iSPNs in homozygous Drd2-eGFP BAC mice is attributable to their increased Drd2 expression.
Drd2 receptors are known to modulate motor function (Albin et al., 1989; DeLong, 1990; Albin et al., 1995; Durieux et al., 2009). To assess non-reinforced ambulatory behavior of mice, an open field test was used. There were no detectable effects of effects of the transgene on ambulatory activity in hemizygous C57BL/6, FVB/N and SW mice (p>0.05, Mann-Whitney U test) (Fig. 5, Table 3). In contrast, in homozygous Drd2-eGFP BAC mice on the FVB/N background, there was a higher level of activity in the corner and periphery of the open field (p<0.05, Mann-Whitney U test), although activity at the center of the arena was not significantly different (Table 3; p>0.05, Mann-Whitney U test). All mice spent the same percentage of time in all regions of the field (p>0.05, Mann-Whitney U test). These assays suggest that anxiety was not affected by transgene zygosity. To pursue this point, fecal droppings were counted (Tache et al., 1993; Henderson et al., 2004). In agreement with the open field data, there was not a significant effect of strain or zygosity on this measure of anxiety (SW WT median = 6.9, n = 8; SW hemi median = 4.3, n =4; FVB/N WT median = 4.8, n = 9; FVB/N homo median = 5.4, n = 9; FVB/N hemi median = 6.1, n = 7; C57BL/6 WT median = 2.5, n = 6; C57BL/6 hemi median = 2.4, n = 5) (p>0.05, Mann-Whitney U test).
BAC transgenic mice have become important tools for neuroscientists, providing a powerful means of dissecting complex neural circuits in the brain (Gong et al., 2003). A critical assumption of studies using these mice is that the transgene does not alter cellular phenotype. Recent work has shown that under some conditions, this assumption is violated (Kramer et al., 2011). Our studies corroborated these important findings. However, this effect was dependent upon mouse strain and transgene zygosity. In commonly used inbred strains of mice (C57BL/6, FVB/N) that were hemizygous for the Drd2-eGFP BAC transgene, there were not significant changes in striatal gene expression, physiology, or motor behavior – justifying the continued use of these mice as reliable tools. This conclusion is similar to that arrived at by another group of investigators studying hemizygous Drd2-eGFP C57BL/6 mice (Nelson et al., 2012).
Our studies examined three different lines of mice – outbred SW, inbred FVB/N and inbred C57BL/6 mice – of varying zygosity for the Drd2-eGFP BAC transgene. Examination of striatal gene expression, striatal physiology and striatally determined behavior revealed that the consequences of transgene expression were dependent upon both strain and zygosity. In agreement with the report of Kramer and colleagues (Kramer et al., 2011), striatal Drd2 and Ttc12 mRNA levels were elevated in striata from hemizygous SW mice. However, expression of none of the other eleven genes assayed was altered in these mice, except VGAT (vesicular GABA transporter). Striatal mRNA for Drd2 and Ttc12 were also elevated in homozygous FVB/N mice and, like SW mice, displayed abnormalities in striatal physiology and open field behavior. Why Drd2 expression was up-regulated in these mice is unclear; one possibility is that having extra copies of the Drd2 intron 2 sequence on the multi-copy BAC array titrates out Freud-1 binding on the endogenous Drd2 gene, leading to increased expression of the endogenous gene (Rogaeva et al., 2007). This effect would have to have a sharp threshold, however, as hemizygous FVB/N and C57BL/6 mice did not display any significant differences in striatal gene expression, physiology or striatally determined behavior attributable to the transgene.
The determinants of this strain dependent variation in response are not clear. However, the impact of strain and subtle variation in gene expression on the response to dopaminergic signaling is very well documented. Differences between strains and rodent species have been described for exploratory and baseline locomotor activity (Miner, 1997; Brodkin et al., 1998; Zamudio et al., 2005; McNamara et al., 2006) and the response to direct and indirect dopaminergic receptor ligands (Severson et al., 1981; Sved et al., 1984; Sanghera et al., 1990; Erwin et al., 1993; Womer et al., 1994; Grahame and Cunningham, 1995; Castellano et al., 1996; Miner, 1997; Brodkin et al., 1998; Patel et al., 1998; Zocchi et al., 1998; He and Shippenberg, 2000; Fowler et al., 2001; McNamara et al., 2006). Differences have also been noted between strains and species in the expression of the DA transporter (Brodkin et al., 1998; Flores et al., 1998; Jiao et al., 2003; Morice et al., 2004; Zamudio et al., 2005; D’Este et al., 2007) and DA receptors (Boehme and Ciaranello, 1981; Severson et al., 1981; Erwin et al., 1993; Ng et al., 1994; Flores et al., 1998; Zamudio et al., 2005; McNamara et al., 2006), as well as differences in DA metabolism (Severson et al., 1981; Sved et al., 1984; Sanghera et al., 1990; Zocchi et al., 1998; He and Shippenberg, 2000), DA cell number (Ross et al., 1976; Baker et al., 1980; Baker et al., 1983; Sved et al., 1984; D’Este et al., 2007), and DA signaling (Ng et al., 1994; Brodkin et al., 1998).
Is the alteration in locomotor behavior with transgene expression attributable to a modest elevation in striatal Drd2 expression, as suggested by Kramer and colleagues (Kramer et al., 2011)? Although plausible based upon current models of striatal function, our studies raise doubts about this conclusion. In hemizygous mice from three different strains (SW, FVB/N, C57BL/6), there was no relationship between striatal Drd2 expression level and open field behavior. While the Drd2 expression from the hemizygous FVB/N and C57BL/6 mice was normal, it was elevated in the hemizygous outbred SW. Our behavioral results are consistent with recent work by Nelson et al. (2012) reporting no behavioral abnormalities in hemizygous Drd2-eGFP C57BL/6 mice. Our results and those of Nelson et al. contrast slightly with those of Ade and colleagues (2011), who found a slight, but significant, elevation in the open field activity of hemizygous Drd2-eGFP mice on a C57BL/6 background.
The basis for the hyperactivity in homozygous Drd2-eGFP BAC FVB/N mice is not clear. It is not readily attributable to an elevation in Drd2 expression. In these mice not only was Drd2 expression elevated, the expression of Drd1a and Adora2a also was above normal. This could reflect a complex cellular and network response to elevated expression of Drd2 in iSPNs or it could be a consequence of insertion effects that have nothing to do with Drd2 per se. Regardless of mechanism, there is a threshold for the effect as hemizygous FVB/N mice were normal in every other assay.
C57BL/6 mice have been the most widely used inbred strain for genetically engineered mice. The FVB/N strain has gained its popularity in this regard for several practical reasons (Hedrich and Bullock, 2004). First, its average litter size is significantly higher than that of other well-known inbred strains. Second, fertilized eggs derived from FVB/N mothers have very large and visually prominent pronuclei; this characteristic greatly facilitates the injection of DNA. Finally, the fraction of injected embryos that survive is also much greater with FVB/N mice than other inbred strains.
A potential problem with inbred colonies is spontaneous mutation, which can lead to drift in the phenotype. There is a consensus that after 20 generations of brother-sister matings, a new inbred line is generated (Silva et al., 1997). For this reason, well-characterized external breeders from established commercial source should be introduced into breeding programs on a regular basis and periodic genotyping performed.
Compared to these inbred strains, outbred strains generally have longer life spans, higher disease resistance and higher overall reproductive performance (Hedrich and Bullock, 2004). Outbred SW mice are well known for their reproductive fitness. However, these outbred strains are genetically heterogeneous making them problematic experimental subjects, particularly if the reproducibility of the response to a subtle intervention is important.
In summary, our studies demonstrate that commonly used inbred strains of mice (C57BL/6, FVB/N) that were hemizygous for the Drd2-eGFP BAC transgene had normal striatal gene expression, physiology, and motor behavior – arguing that these mice provide a reliable tool. Although, the need to use hemizygous mice increases the costs of maintaining a colony, these added costs are offset by the experimental advantages afforded by the mice.
We would like to thank Sasha Ulrich, Karen Saportio, Daniel Kelver, Yu Chen, Lisa Fisher, John Linardakis and Dr. Craig Weiss and for their technical assistance. This work was supported by the Summer Fellowship Program from American Parkinson Disease Association Research to TSG, Summer Fellowship from Parkinson Disease Foundation to QC and REQ, a CHDI contract to DJS, US National Institutes of Health grants NS069777, NS069777-S1 to CSC, and NS34696 to DJS.
Conflict of Interest: none