Amyloid precursor protein (APP) is enriched at the synapse, but its synaptic function is still poorly understood. We previously showed that GABAergic short-term plasticity is impaired in App knock-out (App-/-) animals, but the precise mechanism by which APP regulates GABAergic synaptic transmission has remained elusive. Using electrophysiological, biochemical, moleculobiological, and pharmacological analysis, here we show that APP can physically interact with KCC2, a neuron-specific K+-Cl- cotransporter that is essential for Cl- homeostasis and fast GABAergic inhibition. APP deficiency results in significant reductions in both total and membrane KCC2 levels, leading to a depolarizing shift in the GABA reversal potential (EGABA). Simultaneous measurement of presynaptic action potentials and inhibitory postsynaptic currents (IPSCs) in hippocampal neurons reveals impaired unitary IPSC amplitudes attributable to a reduction in α1 subunit levels of GABAAR. Importantly, restoration of normal KCC2 expression and function in App-/- mice rescues EGABA, GABAAR α1 levels and GABAAR mediated phasic inhibition. We show that APP functions to limit tyrosine-phosphorylation and ubiquitination and thus subsequent degradation of KCC2, providing a mechanism by which APP influences KCC2 abundance. Together, these experiments elucidate a novel molecular pathway in which APP regulates, via protein-protein interaction with KCC2, GABAAR mediated inhibition in the hippocampus.https://doi.org/10.7554/eLife.20142.001
Alzheimer’s disease is the most common form of dementia. One of the hallmarks of the disease is the formation of sticky protein clumps called amyloid plaques in the brain. These plaques are formed from specific fragments of a protein called APP. The intact form of APP is essential for synapses (the junctions across which neurons transmit signals) to form and work correctly.
The hippocampus is one of the first brain regions to be affected in Alzheimer’s disease and is important for forming memories and emotions. In the hippocampus, GABAA receptors at synapses normally tightly regulate synaptic signaling by reducing the ability of the receiving neuron to respond, but this inhibition is disrupted in Alzheimer’s disease. Studies suggest that APP can affect how GABAA receptors transmit signals, but it is not known how it does so. One possibility is that APP regulates a protein called KCC2 that helps to maintain the inhibitory effect of GABAA receptors.
To investigate this, Chen et al. genetically modified mice to lack the gene that produces APP. These mice had a lower level of KCC2 in their hippocampus than normal mice, and their GABAA receptors were less able to inhibit synaptic signaling. Further experiments demonstrated that APP physically interacts with KCC2 and maintains normal levels of the protein by preventing it from being chemically modified and degraded.
Chen et al. also showed that treating mice that lack APP with specific compounds can restore KCC2 activity and return the behavior of synaptic GABAA receptors to normal. Future studies in mice (and eventually people) that exhibit symptoms of Alzheimer's disease will help to determine whether KCC2 is important in the development of the disease. If so, modifying the levels of the KCC2 protein in the brain could potentially help to slow down memory loss in Alzheimer’s disease.https://doi.org/10.7554/eLife.20142.002
APP is a type I single pass transmembrane protein highly expressed in the central nervous system (CNS) which is processed by α-, β-, and γ-secretases (Hardy and Selkoe, 2002) to generate beta amyloid (Aβ) peptide fragments that comprise the amyloid plaques found in Alzheimer’s disease (AD) patients post-mortem. The deleterious impact of Aβ has been studied extensively, with the recent discovery of the potent toxicity of Aβ oligomers on neuronal and synaptic activities (Hsieh et al., 2006; Kim et al., 2006; Wei et al., 2010). Despite advances in our understanding of how Aβ generation drives AD progression, the physiologic role of APP has proven more difficult to elucidate (De Strooper and Annaert, 2000). APP has been detected in vesicular fractions of dendrites and axons (Schubert et al., 1991), suggesting a role for APP in synaptic activity. Moreover, we have shown that APP is required for normal adult neurogenesis (Wang et al., 2014a) and formation of the neuromuscular junction (Wang et al., 2009; Yang et al., 2007).
Many lines of evidence have suggested that APP function can impact the electrophysiological properties of neurons (Kamenetz et al., 2003; Klevanski et al., 2015; Palop and Mucke, 2010; Priller et al., 2006; Selkoe, 2002; Wang et al., 2014a; Yang et al., 2009). Paired-pulse inhibition of GABAergic IPSCs is significantly reduced in App-/- hippocampal slices (Seabrook et al., 1999). However, the molecular mechanism underlying this phenotype is not fully understood. Given that GABAergic function is commonly disturbed in many neuronal disorders including AD (Braat and Kooy, 2015a; Verret et al., 2012), identifying mechanisms whereby APP regulates GABAergic signaling and synaptic inhibition may provide a link between the endogenous function of APP and the etiology of AD.
The K+-Cl- cotransporter, KCC2, is broadly expressed in neuronal membrane of the adult CNS (Kaila et al., 2014). KCC2 functions in setting the proper intracellular Cl- concentration ([Cl-]i) by transporting Cl- against the concentration gradient (Ben-Ari, 2002; Ben-Ari et al., 2012). KCC2 maintains low [Cl-]i in mature neurons, which is essential for maintaining proper postsynaptic inhibition mediated by GABAA receptors (GABAARs) and glycine receptors (GlyRs) (Braat and Kooy, 2015a; Kaila et al., 2014; Rivera et al., 1999). Impaired KCC2 activity and subsequent increases in [Cl-]i occur in several neurological disorders (Boulenguez et al., 2010; Coull et al., 2003; Tang et al., 2016), leading to a depolarizing action of GABAAR mediated currents due to a positive shift of EGABA, and over-excitation of neuronal network activity (Ben-Ari, 2002; Ben-Ari et al., 2012; Blaesse et al., 2009). Recent experiments on KCC2 processing suggest that the intrinsic ion transport rate, cell surface stability, and trafficking of plasmalemmal KCC2 are rapidly and reversibly modulated by the (de)phosphorylation of critical serine and tyrosine residues at the C-terminus of this protein (Lee et al., 2010, 2007). Increased tyrosine phosphorylation of KCC2 leads to enhanced degradation of KCC2 and thus reduced KCC2 protein levels (Lee et al., 2011, 2010). Therefore, abundance of KCC2 protein and the EGABA of a neuron can be regulated by phosphorylation and degradation of KCC2. However, which signaling pathways regulate these phosphorylation events and KCC2 degradation are largely unknown.
In the current study, we aimed to elucidate the synaptic mechanisms underlying APP regulation of hippocampal GABAergic inhibition. We show that APP mediates GABAergic inhibition via a direct protein-protein interaction with KCC2, which stabilizes KCC2 on the cell membrane. APP deficiency causes a loss of acting force holding KCC2 on site, resulting in increased KCC2 degradation via both tyrosine-phosphorylation and ubiquitination, decreased KCC2 levels and, sequentially, a depolarizing shift of EGABA and impairment in GABAAR activities.
In order to test the idea that loss of APP changes the cellular ionic balance of Cl-, thereby altering GABAergic transmission, we used gramicidin perforated patch clamp measurements in acute hippocampal brain slices (Figure 1A) that allows maintenance of an intact intracellular chloride concentration to estimate the IV-relationship of GABAergic currents (Chavas and Marty, 2003). We observed a positive shift of EGABA in App-/- hippocampal CA1 compared to WT controls (WT, −83 ± 6 mV; App-/-, −64 ± 5 mV; p=0.02) (Figure 1B–D), accompanying with identical resting membrane potentials (WT, −61 ± 1.4 mV; App-/-, −59 ± 1.5 mV; p=0.2). We repeated perforated patch recordings in hippocampal cultures and observed a similar depolarizing shift of EGABA in App-/- neuronal cultures (WT, −82.5 ± 4 mV; App-/-, −67 ± 3.8 mV; p=0.02) (Figure 1—figure supplement 1).
Loss of APP impairs GABAergic synaptic transmission (Seabrook et al., 1999; Yang et al., 2009). Given that we see a change in EGABA in hippocampal neurons, we next asked whether loss of APP alters hippocampal IPSCs and GABAAR expression. To do so, we performed dual whole-cell recordings in primary hippocampal cultures. We simultaneously evaluated electrically evoked presynaptic action potentials of a GABAergic interneuron labeled with GAD67+/GFP, while patching a neighboring glutamatergic neuron and recording post-synaptic unitary IPSCs (uIPSCs) at a holding potential of −60 mV (Figure 2A). The mean uIPSC amplitude, evoked by a single presynaptic action potential in the GABAergic neuron, was significantly reduced in App-/- hippocampal cultures compared to WT control cultures (WT, 178 ± 42 pA; App-/-, 80 ± 19 pA; p=0.03) (Figure 2B–C). Similarly, puffing the GABAAR agonist isoguvacine significantly reduced the amplitude of inhibitory currents in App-/- neurons compared to WT neurons (WT, 245 ± 26 pA; App-/-, 146 ± 24 pA; p=0.01) (Figure 2F–G). In contrast, the paired-pulse ratio (PPR) of uIPSCs in response to two consecutive action potentials in GABAergic neurons, at an inter-spike interval of 100 ms and 150 ms to assess synaptic release probability (Zucker and Regehr, 2002), was similar between WT and App-/- (Figure 2D–E) (100 ms; WT, 0.47 ± 0.04; App-/-, 0.56 ± 0.03; p=0.2; 150 ms; WT, 0.51 ± 0.06; App-/-, 0.55 ± 0.05; p=0.75). Consistent with impaired post-synaptic function accounting for these changes in APP mutants, we did not see a decrease in miniature IPSC (mIPSC) frequency, a measure of presynaptic efficacy (Fiszman et al., 2005; Goswami et al., 2012), when we compared App-/- and WT hippocampal slices (Frequency; WT, 2.9 ± 0.8 Hz; App-/- 2.6 ± 0.7 Hz; p=0.8) (Figure 2—figure supplement 1C–D). Meanwhile mIPSC amplitude remained unchanged as well (Amplitude; WT, 14.8 ± 0.4 pA; App-/-, 13.9 ± 0.8 pA; p=0.7) (Figure 2—figure supplement 1C–D). In line with similar frequencies of mIPSCs in WT and App-/- hippocampus, we observed identical numbers of GABAergic neurons in the hippocampus of App-/- and WT mice (Figure 2—figure supplement 1A–B, Figure 2—source data 1). Finally, we looked at the abundance of GABAARs in the hippocampus of APP mutant and WT animals. App-/- hippocampal lysates display reduced immunoreactivity of the α1 subunit, mediating fast inhibition, of the GABAAR but not the other GABAAR subunits, (Figure 2H–I, Figure 2—source data 1). Together, these data suggest that loss of APP may cause postsynaptic deficits in GABAAR mediated GABAergic inhibition.
The electrical response of GABAARs depends on the Cl- equilibrium potential. The best characterized effectors of the Cl- distribution in the CNS are KCC2 and the Na-K-2Cl cotransporter (NKCC1) (Ben-Ari, 2002; Kaila et al., 2014; Lee et al., 2011; Rivera et al., 1999). Since neuronal [Cl-]i is mainly determined by the opposing activities of the Cl- extruding transporter, KCC2, and the Cl- importing NKCC1 (Blaesse et al., 2009), we compared hippocampal KCC2 and NKCC1 levels in WT and App-/- mice. We found that KCC2, but not NKCC1, protein levels were significantly reduced in App-/- hippocampus compared to WT littermate controls (Figure 3A–B, Figure 3—source data 1). KCC2 is mainly localized to the cell surface (Gauvain et al., 2011). To determine whether plasma membrane localization of KCC2 is decreased in APP mutants, we used surface biotinylation in hippocampal tissue (Figure 3A) or HEK293 cells transfected with KCC2 alone or KCC2 and hAPP695 (Figure 3C). We observed significantly reduced plasma membrane KCC2 levels in both App-/- hippocampus and HEK293 cells without co-transfection of hAPP695 (Figure 3B and D, Figure 3—source data 1). To examine KCC2 levels in intact tissue, we performed immunohistochemical staining in slice with anti-KCC2 antibody. We observed a selective loss of KCC2 immunoreactivity in App-/- mice in the CA1 region of the hippocampus (Figure 3E). To determine if this is due to altered transcription of KCC2 in APP mutants, we compared hippocampal KCC2 mRNA levels in App-/- and WT controls. KCC2 mRNA abundance was similar in App-/- and WT hippocampus (Figure 3F, Figure 3—source data 1). Together, these results indicate that APP is required to maintain normal KCC2 protein levels in the hippocampus via a post-transcriptional mechanism.
To determine whether APP could stabilize KCC2 protein, we co-transfected HEK293 cells with KCC2 and hAPP695 cDNAs and assayed subsequent KCC2 protein levels. Cells co-transfected with both constructs displayed higher levels of KCC2 protein compared to cells transfected with only KCC2 (Figure 3G). APP is proteolytically processed into multiple extracellular and intracellular fragments. We tested these fragments individually to determine which fragment conferred KCC2 stability. We transfected HEK293 cells with KCC2+C99, KCC2+sAPPβ, or KCC2+hAPP695. Only full length APP but not the intracellular or extracellular fragments of APP prevented KCC2 degradation (Figure 3H, Figure 3—source data 1). Furthermore, using a sAppβ knock in mouse model (sAppβKi), we observed similarly reduced KCC2 levels in sAppβKi hippocampus compared to WT mice (Figure 3I–J, Figure 3—source data 1). Together, our results indicate that full length APP is required to maintain normal levels of KCC2 protein.
To test whether APP regulates KCC2 through direct protein-protein interaction, we performed immunoprecipitation of KCC2 in HEK293 cells co-transfected with constructs encoding KCC2 and hAPP695. First, Coomassie blue staining was performed in transfected HEK293 cells showing a distribution of all proteins, including APP, pulled down by anti-KCC2 antibody (Figure 4—figure supplement 1). Next, APP was detected in anti-KCC2 immunoprecipitates (IP). Similarly, immunoprecipitation of APP co-precipitated KCC2 (Figure 4A). However, immunoprecipitation of the GABAAR α1 subunit co-transfected with hAPP695, we did not observe a direct physical interaction between APP and GABAAR α1 subunit (Figure 4B). Immunoprecipitation of KCC2 using hippocampal lysates co-precipitated APP as well (Figure 4C). Further, the APP-KCC2 interaction result was strengthened by proximity ligation assay (PLA) which would sensitively detect a very close surface interaction between proteins (Söderberg et al., 2006) (Figure 4D).
KCC2 is regulated post-translationally by tyrosine phosphorylation (Lee et al., 2010; Wake et al., 2007). Increased tyrosine phosphorylation of KCC2 enhances lysozomal degradation and thus decreases KCC2 levels (Lee et al., 2011, 2010). We hypothesized that APP may normally interact with KCC2 to prevent tyrosine phosphorylation and subsequent degradation. To test this hypothesis, we examined whether tyrosine phosphorylated KCC2 levels increased in the absence of APP. Hippocampal tissue from App-/- and WT mice was lysed and immunoprecipitated with anti-KCC2 antibody (Lee et al., 2010). Precipitates were blotted for tyrosine phosphorylated proteins using the anti-P-Tyr antibody, 4G10. We observed a robust increase in tyrosine phosphorylated KCC2 levels in APP mutants compared to littermate controls (Figure 4E). Moreover, total KCC2 protein levels remained decreased in App-/- (Figure 4E) (Relative IOD: WT, 544.86; App-/-, 412.56. hippocampal lysates of three mice per genotype) indicating an increase in tyrosine phosphorylation of KCC2 accompanies the reduction in total KCC2 levels. To further demonstrate that KCC2 instability is due, at least in part, to phosphorylation by a tyrosine kinase in the absence of APP, we tested whether blockade of tyrosine kinases by PP2, a potent inhibitor of Src-family tyrosine kinases (Bi et al., 2000; Lee et al., 2007), enhances KCC2 protein levels. Treatment of HEK293 cells transfected with KCC2 with PP2 at a concentration of 20 µM for 30 min significantly increased KCC2 levels compared to vehicle controls (Figure 4F–G, Figure 4—source data 1). Together, these results suggest that APP-KCC2 interaction functions, at least in part, to limit tyrosine phosphorylation of KCC2, loss of APP leads to excessive tyrosine phosphorylation and premature degradation of KCC2, resulting in reduced KCC2 protein levels in APP mutants.
Next, we tested whether restoring KCC2 function in APP mutant mice would rescue changes in EGABA in hippocampal neurons. Chloride extrusion enhancers, CLP257 and CLP290, have been recently shown to restore Cl- extrusion capacity only in neurons with reduced KCC2 activity (Gagnon et al., 2013). We incubated hippocampal slices from APP mutant mice with CLP257 at 100 µM for 2 hr, and compared EGABA in slices treated with CLP257 or vehicle. Activation of KCC2 in App-/- hippocampus resulted in a hyperpolarizing shift of EGABA (CLP257, −66 ± 3 mV; Control, −54 ± 2 mV; p=0.03) (Figure 5A–B, Figure 5—source data 1). We next tested whether restoration of Cl- extrusion by chronic treatment with CLP290 (Gagnon et al., 2013) rescues KCC2 expression levels. CLP290 or vehicle was intraperitoneally injected once daily for seven consecutive days in App-/- mice, and hippocampal KCC2 levels were analyzed by western blotting. We observed a significant increase in KCC2 levels in CLP290 treated animals compared to vehicle treated App-/- mice (Figure 5C–D, Figure 5—source data 1).
It has been proposed that CLPs might increase KCC2 levels by reducing membrane KCC2 turnover (Gagnon et al., 2013). We then examined, in 293 cells transfected with KCC2, if treatment with CLP257 would indeed increase levels of membrane KCC2, and observed significantly enhanced surface KCC2 levels in CLP257 treated cells compared to vehicle control (Figure 5E–F, Figure 5—source data 1). These experiments could not distinguish whether CLP restored KCC2 levels by increasing insertion or decreasing removal of KCC2. Instead, the study suggested a rescue of KCC2 surface levels and function by CLPs in App-/- mice.
We observed decreases in GABAAR α1 subunit protein levels and smaller evoked IPSC amplitudes in APP mutants (Figure 2). We then tested whether potentiating KCC2 function would rescue GABAAR mediated inhibitory currents in APP mutant hippocampal slices. Evoked whole-cell inhibitory currents, induced by puffing the GABAAR agonist isoguvacine, were recorded after incubation with CLP257 or vehicle for 2 hr, respectively. Evoked inhibitory current amplitudes were significantly larger in CLP257 treated App-/- slices compared to vehicle controls (App-/-: CLP257, 410 ± 34 pA; Vehicle, 278 ± 31 pA; p=0.008) (Figure 5G–H). Importantly, CLP257 treated WT slices did not differ significantly compared to vehicle controls (WT: CLP257, 612 ± 99 pA; Vehicle, 510 ± 109 pA; p=0.5) (Figure 5G–H). Additionally, chronic treatment with CLP290 rescued GABAAR α1 subunit protein levels as well (Figure 5I–J, Figure 5—source data 1). These results support a model in which APP loss of function results in reduced KCC2 levels and decreased KCC2 function, which causes the attenuation of GABAAR α1 expression and GABAAR mediated inhibitory current amplitudes, leading to a decrease of inhibitory tone in the hippocampus of APP mutants.
To test whether GABAAR α1 level changes are dependent on the presence of KCC2, we transfected HEK293 cells with GABAAR α1 or β2 subunits with and without co-transfection of KCC2. Interestingly, we only observed significantly reduced GABAAR α1, but not β2, subunit levels in the absence of KCC2 (Figure 6A–B, Figure 6—source data 1), suggesting a selective role of KCC2 on GABAAR α1 expression.
The mechanisms underlying the actions of KCC2 on GABAergic synapses are currently unclear (Chudotvorova et al., 2005). We next conducted experiments to elucidate how KCC2 regulates GABAAR α1 expression and thus GABAAR mediated inhibition. During immunoprecipitation of the GABAAR α1 subunit co-transfected with KCC2, we did not observe a direct physical interaction between KCC2 and GABAAR α1 subunit (Figure 6C), indicating that KCC2 regulation of GABAAR α1 expression was unlikely through a direct protein-protein interaction.
In a previous report the ubiquitin-like protein PLIC-1, which regulates the membrane trafficking of GABAAR, was shown to directly interact with GABAARs and promote their accumulation at the cell surface (Saliba et al., 2008). We next examined if KCC2 regulates GABAAR α1 levels through affecting PLIC-1 expression, however, Western blotting result showed identical PLIC-1 levels in hippocampus of WT and App-/- mice (Figure 6D–E, Figure 6—source data 1).
It has been shown that expression of GABAAR subunits is regulated by KCC2 expression through affecting intracellular Cl- gradient (Succol et al., 2012). We thus proposed that KCC2-mediated Cl- extrusion might underlie KCC2 regulation of GABAAR α1 protein levels. If this was the case, treatment of WT hippocampus with a KCC2 inhibitor, VU02450551, would result in a reduction of α1 subunit of GABAAR protein levels as seen in App-/- hippocampus. Hippocampal GABAAR α1, several other GABAAR subunits and GluRs levels were analyzed by western blotting after incubation with VU02450551 or vehicle for 2 hr in WT hippocampus slices. We observed a significant decrease in GABAAR α1 levels, but not that of other GABAARs and GluRs subunits in VU02450551 treated WT hippocampus compared to vehicle control (Figure 6F and H, Figure 6—source data 1). Moreover, incubation of App-/- hippocampus with KCC2 inhibitor, VU02450551, further reduced levels of GABAAR α1 subunit but left GluR1 levels unchanged (Figure 6G and H, Figure 6—source data 1). These experiments suggested that blockade of Cl- extrusion by VU02450551 selectively affected levels of GABAAR α1, but not other GABAAR subunits tested in the present study.
It was well known that the expression of KCC2 and GABAergic inhibition parallel neuronal maturation and the emergence of low intracellular Cl- (Ben-Ari et al., 2012; Blaesse et al., 2009; Rivera et al., 1999). KCC2 exports Cl- and is weakly expressed at birth and upregulated as the brain matures (Plotkin et al., 1997; Rivera et al., 1999). To further evaluate the notion that rescue of GABAAR α1 expression and GABAAR mediated inhibition in App-/- hippocampus by restoring KCC2 levels involves alteration in intracellular Cl-, we compared hippocampal KCC2 and GABAAR α1 levels by western blotting in between postnatal day 7 (P7) (with high intracellular Cl- concentration) and P35 (with low intracellular Cl- concentration) WT mice, and observed significantly increased GABAAR and KCC2 levels in P35 compared to P7 hippocampus (Figure 6I–J, Figure 6—source data 1). Similar to western blotting, immunofluorescent staining in P14 and P35 hippocampus displayed higher KCC2 levels in P35 compared to P14 mice (Figure 6—figure supplement 1). Data thus far suggested that rescue of GABAAR α1 levels by restoring KCC2 in App-/- hippocampus involved, at least in part, an alteration of KCC2 mediated Cl- extrusion.
Having shown that one way for APP to regulate KCC2 levels was to limit tyrosine phosphorylation and sequential degradation of KCC2, we speculated that blockade of tyrosine phosphorylation of KCC2 by mutating Y903A and Y1087A (mKCC2) which are two tyrosine phosphorylating sites of KCC2 may restore KCC2 levels in the absence of APP. However, mKCC2 levels were significantly lower without hAPP695 than with (Figure 7A–B, Figure 7—source data 1). Meanwhile, mKCC2 levels are identical in PP2 treated and non-treated HEK293 cells (Figure 7C–D, Figure 7—source data 1) confirming that mKCC2 did not undergo tyrosine phosphorylation, which met desired effect. Moreover, both IP and PLA examinations displayed direct protein-protein interaction between APP and mKCC2 (Figure 7E–F), suggesting that mutation of KCC2 at tyrosine phosphorylating sites did not disturb APP-KCC2 interaction. We then hypothesized that APP deficiency might cause a loss of acting force to hold mKCC2 on site leading to an increase in mKCC2 internalization, resulting in enhanced mKCC2 degradation via an unknown pathway rather than tyrosine phosphorylation. Interestingly, similar to co-transfection of mKCC2 with hAPP695 constructs, HEK293 cells co-transfected with mKCC2 and cylindromatosis (CYLD, a deubiquitinating enzyme) displayed higher levels of mKCC2 protein levels compared to cells transfected with only mKCC2 (Figure 7G–H, Figure 7—source data 1), implicating that mKCC2 might undergo ubiquitination and subsequent degradation in the absence of APP.
Next, treating mKCC2 transfected HEK293 cells (in the presence or absence of APP co-transfection) with the ubiquitination inhibitor MG132, we observed that MG132 increased levels of mKCC2 only in the absence (Figure 8A left–B, Figure 8—source data 1) but not in the presence (Figure 8A right–B, Figure 8—source data 1) of hAPP695, supporting that APP functions to limit mKCC2 ubiquitination. Moreover, using MG132 to block ubiquitination in HEK293 cells transfected with KCC2, we confirmed that ubiquitination occurred in KCC2 as well in the absence of APP (Figure 8C–D, Figure 8—source data 1).
We then examined whether KCC2 ubiquitination contributed to reduction of KCC2 levels in App-/- hippocampus. Hippocampal tissue from App-/- and WT mice was lysed and immunoprecipitated with anti-KCC2 antibody. Precipitates were blotted for ubiquitin/ubiquitinated proteins using the anti-ubiquitin antibody. We observed a robust increase in ubiquitinated KCC2 levels in App-/- hippocampus compared to littermate controls (Figure 8E–F). Furthermore, incubating hippocampus containing App-/- slices with MG132 significantly increased KCC2 levels (Figure 8G–H, Figure 8—source data 1). Moreover, surface KCC2 levels could also be increased by MG132 blockade of KCC2 ubiquitination in HEK293 cells and App-/- hippocampus (Figure 8I–J, Figure 8—source data 1).
Data thus far indicated that KCC2 levels could be regulated post-translationally by ubiquitination as well as tyrosine phosphorylation in the absence of APP. APP-KCC2 interaction played a crucial role in suppressing KCC2 internalization and subsequent degradation via both tyrosine phosphorylation and ubiquitination. APP deficiency resulted in a loss of acting force to hold membrane KCC2, leading to enhanced KCC2 degradation in the hippocampus.
GABA has not only phasic but also tonic mode of action (tonic GABA current) and the latter involves extrasynaptic GABAARs and/or reactive astrocytic GABA (Curia et al., 2009; Jo et al., 2014), and tonic GABA action has been implicated in AD mouse models (Jo et al., 2014; Wu et al., 2014; Yarishkin et al., 2015). We have previously shown that tonic GABA currents were impaired in the dentate gyrus (DG) of App-/- mice attributing to abnormal genesis and survival of DG newborn neurons (Wang et al., 2014b). We thus evaluated whether abnormal tonic GABA currents also occurred in APP deficient CA1 and, observed significantly reduced amplitude of tonic GABA current in the CA1 of App-/- mice compared to WT controls (WT, 19.1 ± 2.7 pA; App-/-, 9.1 ± 0.7 pA; p=0.002) (Figure 9—source data 1). Interestingly, restoring KCC2 by CLP257 incubation of App-/- hippocampal slice did not rescue impaired tonic GABA current (App-/-, 9.1 ± 0.7 pA; App-/-+CLP257, 11.9 ± 1.6 pA; p=0.1) (Figure 9—source data 1), suggesting that aberrant KCC2 levels and function might underlie impaired phasic but not tonic GABA current in the CA1 of App-/- mice.
In this study, we demonstrate that APP regulation of KCC2 expression and function is required to maintain appropriate GABAergic signaling capacity in the hippocampus as summarized in Figure 10. This is supported by several lines of evidence: (1) APP deficiency results in a depolarizing shift of EGABA along with reduced amplitude of uIPSCs and tonic GABA current, (2) APP deficiency results in a significant reduction in the abundance of hippocampal KCC2, but not NKCC1, and GABAAR α1 subunit expression, (3) Phasic GABAergic signaling phenotypes can be rescued by CLPs enhancing KCC2 expression and function, suggesting that impaired regulation of KCC2 by APP is responsible for these fast inhibition deficits in APP mutants, while altered tonic GABA current might involve different mechanisms (Jo et al., 2014; Wu et al., 2014). Together, these data indicate that regulation of KCC2 by APP plays a critical role in the maintenance of normal hippocampal GABAergic inhibition. Identical mIPSC amplitude in between WT and App-/- hippocampus indicates that reduction in GABAAR α1 expression in App-/- does not impair basal inhibitory activity that requires activation of a portion of GABAAR, which is commonly observed when correlating altered receptors with miniature activities (Caraiscos et al., 2004; Chudotvorova et al., 2005).
In previous studies, we have shown that impaired GABAergic short-term plasticity evaluated by abnormal PPR of IPSCs is due, in part, to presynaptic alterations of L-type calcium channels (LTCCs) (Yang et al., 2009). However, we did not see changes in the PPR of uIPSCs in the present study. This may be due to the fact that IPSCs were induced by field stimulation in previous study, which activates multiple presynaptic GABAergic neurons, and corresponding LTCC currents. By contrast, in the present study, uIPSCs were evoked by a single presynaptic action potential in a single GABAergic neuron such that the involvement of presynaptic LTCCs is minimized. This system allowed us to focus on postsynaptic KCC2 dysfunction in APP mutant hippocampal neurons.
KCC2 is the principle mechanism used by neurons to lower internal [Cl-] which is required for adequate inhibitory synaptic transmission upon activation of GABAARs and GlyRs (Braat and Kooy, 2015a; Kaila et al., 2014; Rivera et al., 1999). However, little is known about what regulates KCC2 expression and function. In an attempt to understand why KCC2 levels are diminished in APP mutants, we discovered a physical interaction between APP and KCC2. This interaction protects KCC2 from protein phosphorylation and ubiquitination which target the protein for degradation. These results suggest that APP is a novel protein binding-partner for KCC2. APP holds KCC2 on membrane through protein-protein interaction to maintain appropriate KCC2 levels, internal Cl- and GABAAR mediated inhibition. Though increased activation of glutamatergic receptors has been shown to downregulate KCC2 expression and GABAAR mediated current (Lee et al., 2011), neither amplitude, frequency of mEPSCs (Amplitude; WT, 13.3 ± 0.4 pA; App-/-, 12.6 ± 0.8 pA; p=0.5; Frequency; WT, 0.2 ± 0.05 Hz; App-/- 0.4 ± 0.2 Hz; p=0.3) nor GluRs protein levels changed in hippocampus of APP mutants compared to WT controls (Figure 2—figure supplement 2A–D, Figure 2—source data 1). The results suggest that excitatory synaptic activity mediated by AMPA receptors may not be affected by loss of APP at the age tested.
Changes in KCC2 levels that occur in APP mutants can have wide ranging effects on the status of GABAergic signaling. Modulation of KCC2 protein levels has been reported to affect GABAAR density and GABAergic inhibition (Chudotvorova et al., 2005; Succol et al., 2012). Therefore, we postulated that altered KCC2 function in APP mutants accounts for changes in GABAergic signaling. To test this, we pharmacologically enhanced KCC2 function in App-/- mice and observed a rescue in both amplitudes of isoguvacine induced currents and GABAAR α1 expression levels, indicating a rescue of GABAergic functional deficits by restoring KCC2 function. Moreover, we show that blockade of KCC2 mediated Cl- extrusion in WT hippocampus resulted in a reduction of GABAAR α1 levels as seen in App-/- mice and, GABAAR α1 levels are positively correlated with KCC2 expression and function during early stage of development. We thus reasoned that increase in KCC2 mediated Cl- extrusion might be responsible for upregulation of surface GABAAR α1 levels.
Though the exact mechanism underlying how restoring KCC2 rescued surface GABAAR α1 levels remains unclear, given that APP interacts directly with KCC2, and increasing KCC2 expression and function rescued GABAergic signaling phenotypes in App-/- hippocampus, we propose that KCC2 is the primary defect caused by APP deletion to alter GABAergic signaling, while changes in GABAAR α1 levels and GABAAR mediated inhibition are secondary to altered KCC2 expression and function.
Our results indicate that full length APP is required to maintain normal levels of KCC2 protein. Together with a recent study of the AppΔCT15-DM mice, a mouse model lacking the last 15 amino acids of APP as well as the APP homologue, APLP2, which demonstrated impairments of synaptic plasticity and hippocampal-dependent behavior (Klevanski et al., 2015), it is likely that APP proteolysis may be a mechanism for turning off normal APP functions which needs to be taken into account when exploring the pathophysiology of APP with respect to KCC2 regulation.
GABAergic signaling has been shown to be disrupted in many diseases of the nervous system (Braat and Kooy, 2015a), including fragile X syndrome and autism spectrum disorder (Braat and Kooy, 2015b; Han et al., 2014). Changes in KCC2 function may account for many GABAergic signaling deficits, as it has been shown to be involved in the pathogenesis of epilepsy, schizophrenia, autism and aging brain (Ben-Ari et al., 2012; Ferando et al., 2016; Tang et al., 2016; Tao et al., 2012). Though the GABAergic system appears to be resistant to Aβ toxicity (Selkoe, 2002), recent research has demonstrated dysfunctional GABAergic inhibition in AD (Verret et al., 2012). In the present study, we have described a cellular mechanism by which loss of APP function downregulates KCC2 to impair GABAergic signaling. Given the results presented here in APP mutant hippocampal neurons, if APP function is compromised in the context of progressing AD, this may lead to the gradual loss of GABAergic signaling capacity in the hippocampus and associated changes in memory function. Together with a most recent study revealing a critical role of KCC2 in information storage in aging brain (Ferando et al., 2016), the present study suggests that KCC2 might serve as a therapeutic target to improve GABAergic inhibition to potentially restore hippocampal function and improve memory in AD.
All experiments and animal housing were in accordance with procedures approved by the Ethics Committee for animal research at South China Normal University, according to the Guidelines for Animal Care established by the National Institute of Health. Both female and male mice were used in this study. App-/- and wild type (WT) mice (Zheng et al., 1995) were generated by crossing App+/- males and females obtained from Model Animal Research Center of Nanjing University (Nanjing, China). App-/- mice were crossed with Gad67+/GFP mice (Tamamaki et al., 2003) (gift from Dr. Yuqiang Ding at Tongji University School of Medicine, Shanghai, China) when necessary to generate App-/--Gad67+/GFP and WT-Gad67+/GFP controls. Soluble APP ectodomain beta (sAppβ) knock in mice (Li et al., 2010), full length human APP (hAPP695), APP C-terminal fragments (C99) and sAPPβ constructs were from Hui Zheng lab at Baylor College of Medicine. The KCC2 construct was gift from John A Payne (School of Medicine, University of California). The GABAAR α1 construct was gift from Gangyi Wu (South China Normal University, Guangzhou, China). CYLD construct was gift from Shaocong Sun (University of Texas MD Anderson Cancer Center, Texas, USA). GABAAR β2 construct was from Yong Zhang (Peking University).
Cultured hippocampal neurons were prepared as described (Yang et al., 2009) with some modifications. Briefly, we dissected hippocampus from App-/--Gad67+/GFP and WT-Gad67+/GFP littermates of P0/1 pups, trypsinized the tissue at 37°C for 30 min, and then gently triturated in culture medium containing 10% heat-inactivated fetal bovine serum using fire-polished pipettes, before centrifuging at 1000 rpm for 10 min. Cells were resuspended in Neurobasal Medium supplemented with B27 and L-glutamine (Invitrogen, Carlsbad, CA), and plated at 1–2 × 104 cells/ml onto 13 mm poly-L-lysine coated coverslips. One day after plating, 4 M cytosine-D-arabinofuranoside (Ara-C) (Sigma) was added to prevent astrocyte proliferation. Cultures of 12–14 DIV were used for patch clamp recordings.
Hippocampal slices (350 μm thick) were cut using a vibratome (LeicaVT1000S) in ice-cold cutting solution containing the following: 25 mM NaHCO3, 2.5 mM KCl, 7 mM MgCl2, 1.25 mM NaH2PO4, 7 mM Glucose, 0.5 mM CaCl2, 115 mM Choline Cl. Slices were incubated for 45 min in artificial cerebrospinal fluid (aCSF) solution containing the following: 119 mM NaCl, 2.5 mM KCl, 2.5 mM CaCl2, 1.3 mM MgSO4, 1 mM NaH2PO4, 11 mM D-glucose, 26.2 mM NaHCO3. Pipettes were filled with an internal solution of 136.5 mM K-Gluconic acid, 17.5 mM KCl, 9 mM NaCl, 1 mM MgCl2, 0.2 mM EGTA, 10 mM HEPES (pH 7.3) containing gramicidin A 10 μg/ml (Sigma; diluted from a stock solution of 10 mg/ml in DMSO). The recording aCSF contains: 140 mM NaCl, 4.7 mM KCl, 2.5 mM CaCl2, 1.2 mM MgCl2, 11 mM D-glucose, 10 mM HEPES (pH 7.3). Both incubating and recording solutions were bubbled with 95% O2 and 5% CO2 throughout the experiment. We performed all the experiments for the determination of EGABA values in the presence of TTX (1 μM), CNQX (20 μM), APV (50 μM) and Strychnine (1 μM) to block voltage-gated sodium channels, AMPA receptors, NMDA receptors, and GlyRs, respectively. A Picospritzer (Parker Instrumentation) was used to eject GABA (100 μM, 100 ms) directly onto neuronal soma through a fine pipette (~2 μm tip). For mEPSC and mIPSC recordings, the aCSF was supplemented with 1 μM TTX, and pipettes were filled with an internal solution of 100 mM Cs gluconate, 5 mM CsCl, 10 mM HEPES, 2 mM MgCl2, 1 mM CaCl2, 11 mM BAPTA, 4 mM ATP, 0.4 mM GTP. To record tonic GABA current, 10 μM CNQX and 50 μM APV were added into the aCSF to block glutamate receptors. The total tonic GABA current was revealed by the change of holding current after perfusion of 100 μM bicucullin (Bic). Pipettes were filled with an internal solution of 135 mM CsCl, 5 mM Na-phosphocreatine, 10 mM HEPES, 5 mM EGTA, 4 mM MgATP, 5 mM QX-314 and 0.5 mM Na2GTP (pH 7.3) (Wu et al., 2014). Data were filtered during acquisition with a low pass filter set at 2 kHz using pClamp10 (Molecular Devices). Data analysis was performed offline with Clampfit 10.2 (Molecular Devices).
GABA reversal potential recordings were made using a perforated patch-clamp technique. Pipettes were filled with an internal solution of 140 mM KCl and 10 mM HEPES (pH 7.3) containing gramicidin A 50 μg/ml (Sigma; diluted from a stock solution of 50 mg/ml in DMSO). Data were filtered during acquisition with a low pass filter set at 2 kHz using pClamp10 (Molecular Devices). Data analysis was performed offline with Clampfit 10.2 (Molecular Devices).
The culture coverslips were transferred into a heated (30°C) submerged recording chamber, continuously perfused (2–3 ml/min) with tyrode buffer: 129 mM NaCl, 5 mM KCl, 0.01 mM Glycine, 1 mM MgCl2, 2 mM CaCl2, 25 mM HEPES, 30 mM D-Glucose. We performed all experiments for the determination of unitary inhibitory postsynaptic current (uIPSC), and paired-pulse ratio (PPR, uIPSC2/uIPSC1) values in the presence of CNQX (20 μM) and APV (50 μM) to block AMPA receptors and NMDA receptors, respectively. GABAergic neurons were patched in whole-cell, current-clamp configuration using an Axopatch 700B amplifier (Axon Instruments) Channel 1. The pipette solution contained 110 mM K-Gluconic acid, 10 mM NaCl, 1 mM MgCl2, 10 mM EGTA, 40 mM HEPES, 2 mM ATP, 0.3 mM GTP (pH adjusted to 7.2 with NaOH). Pyramidal neurons were patched in voltage-clamp configuration and recorded at a holding potential of −60 mV using an Axopatch 700B amplifier (Axon Instruments) Channel 2. The pipette solution contained 100 mM Cesium Methanesulfonate, 10 mM NaCl, 10 mM TEA-Cl, 1 mM MgCl2, 10 mM EGTA, 40 mM HEPES, 2 mM ATP, 0.3 mM GTP, 4 mM QX-314 (pH adjusted to 7.2 with NaOH). Before uIPSC recordings, voltage responses of presynaptic and postsynaptic cells were recorded by applying long hyperpolarizing and depolarizing current pulse (300 ms) injections to examine basic electrophysiological properties, including input resistance, single spike kinetics, voltage-current relationships, repetitive firing patterns, and firing frequency. For evoked GABA current recording, a Picospritzer (Parker Instrumentation) was used to eject isoguvacine (100 μM, 100 ms) directly onto neuronal soma through a fine pipette (~2 μm tip).
Mice brains were dissected and immediately frozen in liquid nitrogen. Total RNA was extracted using Trizol reagent. RNA pellets were resuspended in diethylpyrocarbonate-treated water and RNA concentration was measured using a Nanodrop2000c spectrometer (Thermo Scientific). RNA was DNase treated (DNase I, amplification grade, Invitrogen) and then reverse-transcribed using the Superscript III First-Strand Synthesis System (Invitrogen). Relative quantification of gene expression was performed using Taq Manprobes and an ABI Prism 7000 Sequence Detection System. Platinum Quantitative PCR Super Mix-UDG w/ROX (Invitrogen) was used with the following primers and probes: App F-primer, (5’–3’) CCAAGAGGTCTACCCTGAACTGC; App R-primer, (5’–3’) AGGCAACGGTAAGGAATCACG; Actβ F-primer (5’–3’) GTGACGTTGACATCCGTAAAGA; Actβ R-primer (5’–3’) GTAACAGTCCGCCTAGAAGCAC; Slc12a5 F-primer (5’–3’) GGGCAGAGAGTACGATGGC; Slc12a5 R-primer (5’–3’) TGGGGTAGGTTGGTGTAGTTG. Assay efficiencies were experimentally determined using a five-point dilution series of cDNA spanning a 100-fold range in concentration. 0.025 µg cDNA template was used per reaction. Statistical analysis was performed on 2-∆∆Ct values.
Mice were anesthetized with intraperitoneal injection of 20% urethane (0.01 ml/g) and perfused transcardially with 0.9% physiological saline and 4% paraformaldehyde (PFA) in phosphate buffer (0.01 M PBS, pH 7.4). Following perfusion, the brains were dissected and post-fixed overnight in 4% PFA followed by a sucrose series (10%, 20% and 30%) solution at 4°C for cryoprotection. Serial coronal/sagittal sections of tissue were obtained using Lycra frozen slicer 1800 with a thickness of 30 μm. Free-floating sections were rinsed in PBS three times for 5 min and processed for antigen retrieval by boiling in 10 mM citrate buffer (pH 6.0) for 5 min. The sections were incubated in 3% H2O2 in PBS for 15 min at room temperature (RT) to quench endogenous peroxidases, washed three times for 5 min and subsequently incubated in 0.3% Triton X-100 in PBS for 2 hr. To block nonspecific binding, sections were incubated in 3% bovine serum albumin (BSA) for 30 min. Sections were then incubated overnight with primary antibody against KCC2 (Neuromab, 75–013; Millipore, 07–432) at 4°C. After three washes with PBS, secondary antibody (CWS) application was performed at RT for 2 hr followed by three additional washes with PBS for 10 min. The secondary antigen was visualized with 3,3-diaminobenzidine tetrahydrochloride (DAB, Sola). The reaction was terminated by rinsing in PBS and then sections were mounted on gelatin-subbed slides, dehydrated in ascending alcohol concentrations, cleared through xylenes, and covered with DPX resin. KCC2 immunofluorescent staining was conducted as described (Yang et al., 2009).
Mouse brains were homogenized using SDS lysis buffer (50 mM Tris pH 7.5, 150 mM NaCl, 5 mM EDTA pH 8.0, 1% SDS) containing complete protease inhibitor cocktail (Roche). After 1 min of homogenization, the cellular debris was removed by centrifugation at 14000 rpm for 10 min at 4°C and supernatant was collected and denatured for 20 min at 75°C. Tissue lysates were subjected to SDS-PAGE (Bio-Rad) and transferred to nitrocellulose membranes. Membranes were blocked for 0.5 hr using 5% non-fat dry milk in TBS containing 0.5% Tween-20 (TBST), then incubated with specific primary antibodies against KCC2 (Neuromab, 75–013; Millipore, 07–432; Santa Cruz, sc-19419), NKCC1 (Abcam, ab191289), APP (Abcam, ab15272), 4G10 (Millipore, 16–452), PLIC-1 (ABGENT, AP2176c), GABAAR subunits: α1 (Millipore, 06–868), α5 (Abcam, ab175195), β2 (Abcam, ab156000), δ (Abcam, ab110014), γ2 (Abcam, ab87328), GluR1 subunit (Abcam, ab31232) and GluR2 subunit (Abcam, ab206293) of AMPA receptors, and ubiquitin (Abcam, ab7254). Anti γ-tubulin antibody (Sigma, T6557) was used as a loading control. Antibodies were diluted at 1:1000 to 1:2000 at use. After three washes with TBST, secondary antibody (CWS) application was performed at RT for 1 hr using 5% milk in TBST followed by three additional washes with TBST. Bands were visualized using Immobilon Western ECL system and analyzed with Gel Pro Analysis software. For surface KCC2 detection, biotinylation of cell surface proteins was performed as described previously (Lee et al., 2010). Briefly, HEK293 cells transfected with KCC2 constructs or cultured neurons were washed two times with PBS containing 0.5 mM MgCl2 and 1 mM CaCl2 (PBS-CM) and then incubated with 2 ml of PBS-CM containing 1 mg/ml Sulfo-NHS-SS-Biotin (Pierce) for 30 min at 4°C. After labeling, the biotin reaction was quenched by washing three times with ice-cold PBS-CM containing 50 mM glycine and 0.1% BSA. Cells were then lyzed with 1 ml lysis buffer and the lysate was collected. Protein concentration was determined using Micro BCA protein assay kit (Thermo Scientific). After correction for protein concentration, 40 μl of 1:1 slurry of UltraLink NeutrAvidin (Pierce) was added to the lysates to pull down the biotin-labeled surface proteins for 2 hr at 4°C. The NeutrAvidin beads were washed and bound materials were analyzed by SDS-PAGE.
To obtain a KCC2 plasmid in which the tyrosine phosphorylating sites, Y903A and Y1087A, were mutated (mKCC2), the KCC2 open reading frame (ORF) was amplified from the pCAGIG vector, incorporate Y903A and Y1087A mutation using the stratagene QuickChange method as described (Lee et al., 2010). For mutation of Y903 the following primers were used: (sense) TCCGGATCCACTCGAGATGCTCAAC; (antisense) AATGTCTTCTCGAAGGTG TATGCTG. For mutation of Y1087 the following primers were used: (sense) TACACCTTCGAGAAGACATTGG; (antisense): ATTTACGTAG CGGCCGCTCAGGAGT AGATGGATATCTGCAGAATTCCATGAAGTTTTCATCTCC.
Commercially-available HEK293 cells, original transformated as reported (Graham et al., 1977), were co-transfected with KCC2 and GABAAR α1 or β2; KCC2 and APP/ or different APP fragments. Whenever necessary, KCC2 was replaced by mKCC2. Transfected HEK293 cells were washed with ice-cold PBS, centrifuged at 5000 rpm for 10 min at 4°C, and the precipitate was collected and homogenized using SDS lysis buffer, centrifuged at 14,000 rpm for 10 min at 4°C and supernatant and denatured for 20 min at 75°C. Supernatants were analyzed by western blotting.
HEK293 cells were grown in DMEM (high glucose with L-glutamine) containing 10% FBS. For immunoprecipitation, HEK293 cells were plated onto 10 cm culture dishes, and grown to 70% confluency. Cell transfections were performed with lipofectamine 2000 (Invitrogen), following the manufacturer’s recommended protocol. 24–48 hr after transfection, cells were washed once with cold PBS then homogenized with 1 ml cold lysis buffer (50 mM Tris pH 7.5, 150 mM NaCl, 1 mM EDTA, 1% NP40, and protease inhibitor) in 2 ml tubes. To remove cell debris, lysates were centrifuged for 20 min at 14,000 rpm at 4°C. Supernatants were incubated with 2 μl of KCC2 (Millipore, 07–432), APPc (Wang et al., 2007), or GABAAR α1 (Millipore, 06–868), antibodies at 4°C overnight. Protein A agarose beads at 30 μl (Millipore) was added to each sample and they were incubated at 4°C for 2–3 hr. To control for nonspecific binding, protein lysates incubated with rabbit or mouse IgG and beads were processed in parallel. Subsequently, beads were washed three times with 500 μl of cold lysis buffer. Immunoprecipitates were eluted from the beads by adding 30 μl of SDS-PAGE sample buffer and heating for 20 min at 75°C. The eluates (15 μl) were analyzed by western blotting. For hippocampal lysates immunoprecipitation, we followed the HEK293 cells protocol above. Coomassie blue staining was conducted as described (Savas et al., 2015).
HEK293 cells were grown in DMEM containing 10% FBS. For PLA (Söderberg et al., 2006), HEK293 cells were plated onto 10 cm culture dishes, and grown to 70% confluency. On the day of experiment, the wells were washed with 1xPBS and then added with 4% PFA and incubated for 10 min at RT without agitation. Then the cells were washed with PBS for 3 times, 5 min each, with agitation and treated with 0.5% Triton X-100 in PBS (PBST) for 10 min without agitation. Wash the cells with TBST for 3 times, 5 min each, with agitation. Block with Duolink II Blocking Solution (1x) for 1 hr at 37°C and then incubate with specific primary antibodies against KCC2 (Neuromab, 75–013) or APP (Abcam, ab15272). After wash with 1x Duolink II Wash Buffer A, cells were incubated with two PLA probes (Duolink II anti-Mouse MINUS and Duolink II anti-Rabbit PLUS) 1:5 in Antibody Diluent. Wash the slides in 1x Wash Buffer A for 2 times, 5 min each, with agitation at RT. Incubate the slides with Ligation-Ligase solution for 30 min at 37°C. Wash the slides in 1x Wash Buffer A with for 2 times, 2 min each. Then incubate the slides with Amplification-Polymerase solution for 100 min at 37°C. Wash the slides for 2 times, 10 min each, in 1x Duolink II Wash Buffer B and incubate with DAPI for 15 min at 37°C. Data was analyzed with a fluorescence microscope.
KCC2 enhancers, CLP257 and CLP290 (Gagnon et al., 2013) were gifts from Yves De Koninck (Institut universitaire en santé mentale de Québec, Qc, Canada).
CLP257 incubation: CLP257 was dissolved in 200 µl DMSO as 100 mM stock solution and diluted using aCSF to 100 µM. For slice recording, hippocampal slices (350 μm thick) of App-/- mice were cut using a vibratome (LeicaVT1000S) as described above for whole-cell recording in acute hippocampal slices. Slices were incubated for 2 hr in aCSF containing 100 μM CLP257 or DMSO and babbled with 95% O2 and 5% CO2. For surface and total KCC2 protein levels evaluation, HEK293 cells, which was transfected with KCC2 were incubated for 2 hr in 100 μM CLP257 or DMSO.
CLP290 intraperitoneal injection: CLP290 was dissolved in HPCD and intraperitoneally administered once daily at a dose of 100 mg/kg for one week. HPCD injection group was used as vehicle control.
Unless otherwise stated, data are displayed as mean±SEM. Student’s t-test was used for statistical analysis in two-group comparison. For comparison among multiple groups, one-way ANOVA or two-way ANOVA with post hoc tests were used. Statistical significance was set at p<0.05.
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Eunjoon KimReviewing Editor; Institute for Basic Science, Korea Advanced Institute of Science and Technology, Republic of Korea
In the interests of transparency, eLife includes the editorial decision letter and accompanying author responses. A lightly edited version of the letter sent to the authors after peer review is shown, indicating the most substantive concerns; minor comments are not usually included.
Thank you for submitting your article "APP is a novel protein-binding partner for KCC2: An insight on the role of APP in hippocampal GABAAR mediated inhibition" for consideration by eLife. Your article has been favorably evaluated by a Senior Editor and three reviewers, one of whom is a member of our Board of Reviewing Editors. The following individual involved in review of your submission has agreed to reveal his identity: C Justin Lee (Reviewer #2).
The reviewers have discussed the reviews with one another and the Reviewing Editor has drafted this decision to help you prepare a revised submission.
This study provides some evidence that APP stabilizes KCC2, a K+-Cl- cotransporter, on the cell surface and that APP regulates GABAA receptor-mediated synaptic transmission. The authors first showed the GABA reversal potential shifts toward depolarization, the decreased unitary IPSC amplitude, and the reduced GABAA receptor protein level in the hippocampus of APP-/- mice. Then, the authors found that APP directly binds to KCC2 and prevents KCC2 from its degradation. Furthermore, the authors showed that restoration of KCC2 function in APP-/- mice by CLP290 rescues GABAA receptor levels and function. Because patho-physiological functions of APP have attracted considerable attention, this work addresses a generally important topic. Addressing the following points would strengthen this paper.
1) The authors provide data suggesting that KCC2 in the absence of APP is degraded through ubiquitin-dependent mechanisms and enhanced endocytosis. However, the data supporting this conclusion mainly presented in Figure 6 are very weak. Specifically, there is no evidence supporting that APP2 deficiency causes KCC2 ubiquitination or KCC2 endocytosis. In addition, it is unclear whether endocytosis of KCC2 is functionally coupled to ubiquitination.
2) Although the link between APP and KCC2 is abundantly clear, the link between KCC2 and GABAA is not so clear. For example, in Figure 1 and Figure 1—figure supplement 1 there appears to be a significant difference in Egaba between WT and APP-/-. However, there appears to be a difference in the conductance (slope of the IV) between whole cell (Figure 1) in slice and perforated patch (Figure 1—figure supplement 1) in culture. This type of discrepancy is also shown in Figure 2—figure supplement 1, in which the amplitude of mIPSC for WT and APP-/- did not show the expected difference. These discrepancies might be due to the fact that authors apparently do not fully address the field of GABA inhibition. GABA has not only phasic mode but also tonic mode of action. In recent studies, tonic GABA release from reactive astrocytes and its inhibitory action has been implicated in Alzheimer's disease (Jo, et al., 2012; Wang, et al., 2012; also, see Yarishkin et al., 2015). KCC2 could not only affect synaptic GABAA receptors but also extrasynaptic GABAA receptors. In addition, isoguvacine which is used for monitoring functional surface GABAA activates not only synaptic GABAA but also extrasynaptic GABAA, complicating authors' interpretations. Therefore, authors need to introduce the current state of phasic and tonic GABA appropriately and discuss their results accordingly.https://doi.org/10.7554/eLife.20142.026
- Cheng Long
- Li Yang
- Cheng Long
- Li Yang
- Cheng Long
- Li Yang
- Cheng Long
- Li Yang
- Li Yang
- Li Yang
The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.
The authors thank Dr. Yasunori Hayashi for suggestions on the manuscript; Zhijie Zhang for technical support. This work was supported by grants from the National Natural Science Foundation of China (31171018, 31171355), the Science and Technology Division of Guangdong (2013KJCX0054, 201607010320), and the Natural Science Foundation of Guangdong Province (2014A030313418, 2014 A030313440).
Animal experimentation: This study was conducted along the guidelines described in "The Guide for the Care and Use of Laboratory Animals" (Eighth Edition). All of the animals were handled according to approved institutional animal care and use committee (IACUC) protocols (#0312-11) of the South China Normal University. Every effort was made to minimize suffering.
- Eunjoon Kim, Reviewing Editor, Institute for Basic Science, Korea Advanced Institute of Science and Technology, Republic of Korea
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