Amyloid precursor protein modulates β-catenin degradation
© Chen and Bodles; licensee BioMed Central Ltd. 2007
Received: 02 October 2007
Accepted: 10 December 2007
Published: 10 December 2007
The amyloid precursor protein (APP) is genetically associated with Alzheimer's disease (AD). Elucidating the function of APP should help understand AD pathogenesis and provide insights into therapeutic designs against this devastating neurodegenerative disease.
We demonstrate that APP expression in primary neurons induces β-catenin phosphorylation at Ser33, Ser37, and Thr41 (S33/37/T41) residues, which is a prerequisite for β-catenin ubiquitinylation and proteasomal degradation. APP-induced phosphorylation of β-catenin resulted in the reduction of total β-catenin levels, suggesting that APP expression promotes β-catenin degradation. In contrast, treatment of neurons with APP siRNAs increased total β-catenin levels and decreased β-catenin phosphorylation at residues S33/37/T41. Further, β-catenin was dramatically increased in hippocampal CA1 pyramidal cells from APP knockout animals. Acute expression of wild type APP or of familial AD APP mutants in primary neurons downregulated β-catenin in membrane and cytosolic fractions, and did not appear to affect nuclear β-catenin or β-catenin-dependent transcription. Conversely, in APP knockout CA1 pyramidal cells, accumulation of β-catenin was associated with the upregulation of cyclin D1, a downstream target of β-catenin signaling. Together, these data establish that APP downregulates β-catenin and suggest a role for APP in sustaining neuronal function by preventing cell cycle reactivation and maintaining synaptic integrity.
We have provided strong evidence that APP modulates β-catenin degradation in vitro and in vivo. Future studies may investigate whether APP processing is necessary for β-catenin downregulation, and determine if excessive APP expression contributes to AD pathogenesis through abnormal β-catenin downregulation.
β-Catenin plays a central role in Wnt signalling in the canonical pathway . In the absence of Wnt signalling, cytoplasmic β-catenin exists in a complex together with axin, adenomatous polyposis coli (APC), and glycogen synthase kinase (GSK)-3β. GSK-3β constitutively phosphorylates β-catenin at Ser33, Ser37, and Thr41 (S33/37/T41) residues, triggering ubiquitinylation by a Cullin-1-containing E3 ligase (also known as the SCF complex) before proteasomal degradation [2–6]. Signalling by Wnt through Frizzled and LRP cell surface receptors inhibits GSK-3β and stabilizes β-catenin. When stabilized, β-catenin translocates to the nucleus and functions as a transcription cofactor of the T cell factor (TCF), activating responsive genes such as cyclin D1 and c-myc.
Several lines of evidence suggest that APP influences β-catenin regulation. APP binds to APP-BP1 which activates the small ubiquitin-like protein Nedd8 [7, 8]. Activated Nedd8 modifies Cullins which then becomes more stable. When Cullin-1 in SCF is transiently stabilized, it increases β-catenin ubiquitinylation and degradation . In addition, APP plays an important role in cell-cell adhesion , a function that may involve β-catenin. Membrane-associated β-catenin anchors cadherins to the actin cytoskeleton . Interactions with cadherins may underlie an important role for β-catenin in synaptic integrity of neurons . Synaptic dysfunction is one of the earliest events in AD pathogenesis , and APP appears to contribute to synapse formation or stabilization [14–16].
Both APP and Presenilins are genetically associated with AD. In addition to its role in APP processing, Presenilin-1 (PS1) also interacts with the cadherin/catenin adhesion complex  and affects β-catenin delivery to the membrane adhesion complex . There is some controversy surrounding the influence of PS1 and its FAD mutants on β-catenin [19–26]. Similarly, different levels of β-catenin have been reported in AD [27–29]. This is likely attributable to the complexity of these systems made possible by multimodal interactions between APP, PS1, β-catenin, and E-cadherin; a complexity that justifies more detailed analyses of these systems. The purpose of this report is to determine whether APP mediates β-catenin degradation in vitro and in vivo. We provide critical evidence that APP downregulates β-catenin in neurons.
Pregnant Sprague-Dawley rats (E18, Charles River, Wilmington, MA) were euthanized after being rendered unconscious with CO2 according to the protocol approved by the Institutional Animal Care and Use Committee. The cortices from embryonic brains were gently triturated with a fine-tipped transfer pipette right after dissection. Single cells were counted and immediately plated in Neurobasal medium containing B27 supplements (Invitrogen, Calsbad, CA), 0.5 mM glutamine, 1% FBS, 1% equine serum, and 1× penicillin/streptomycin (Sigma, St. Louis, MO) at a density of 4 × 106 per 60-mm dish or 4 × 105 per well of 24-well plate on poly-D-lysine-coated dishes. The medium was replaced with fresh medium at 2 h after plating. Half of the medium was replaced with fresh medium every three days. The adult rat brain and other organs were dissected and frozen on dry ice before lysis and immunoblot analyses. Primary neurons were used at 7 DIV unless noted otherwise.
HSV expression vectors and viral titers
Constructs of full length APP (APP695), mycAPP-BP1, and LacZ (expresses β-galactosidase) in the pHSVprPUC vector [7, 30] were packaged into HSV-1 virus using the 2-2 cell line as described by Lim et al. . Each viral stock infectious unit (IU) was determined by counting ten randomly selected fields of infected primary neurons immuno-stained for APP and myc tag, or cytochemically stained for β-galactosidase using X-gal substrate (Roche).
Short hairpin RNA (shRNA)
RNA interference was achieved via shRNAs expressed from the pHSVGET vector for neuronal expression . Each shRNA duplex was designed with a TCA AGA G loop. The APP shRNA was targeted to the following sequence: 5'-GCA GAA GAT GTG GGT TCA AAC-3' (APP1996). The control shRNA included the missense sequence 5'-GCT TCA TAA GGC GCA TAG CTA-3'. In some experiments, the vector pHSVGET was used as a control. All constructs were sequenced before HSV viral packaging. Viruses were packaged as described . The IU of each shRNA virus was determined by the number of EGFP-expressing cells after infecting primary neurons for 15 hours. EGFP-positive cells were visualized by fluorescence microscopy after fixation in 4% paraformaldehyde for 15 min at room temperature.
Neuron infection, western blots, and antibodies
For all western blot analyses, primary neurons in 60-mm dishes were infected at 7 DIV with 1 or 2 IU per cell (for protein expression), or at 0.5 or 1 IU per cell (for shRNA knockdown analyses). At 14–15 h after infection, cells were washed with cold phosphate-buffered saline (PBS) and sonicated in lysis buffer (150 mM NaCl, 50 mM sodium fluoride, 50 mM Tris-HCL, 10 mM β-glycerol phosphate, 5 mM EDTA, 5 mM iodoacetamide, 1 mM phenylmethylsulfonylfluoride, 1 mM sodium orthovanadate, 1% NP-40, 0.5% sodium deoxycholate, 0.1% SDS, pH 8.0). Protein concentrations were determined by the bicinchronic acid (BCA) method; equal amount of protein was boiled in SDS sample buffer and resolved on SDS-PAGE gels. The following antibodies were used: rabbit anti-β-catenin and mouse anti-γ-tubulin (both from Sigma); anti-phosphorylated β-catenin antibodies, S33/37/T41 and S45 (both from Cell Signaling); rabbit anti-APP antibody (369, a gift from Dr. Sam Gandy). Chemiluminescence reactions were carried out using ChemiGlow (Alpha Innotech) and the blot digital images were collected by the AlphaEase FC™ Imaging System and the FluorChem™ IS-8800 software (Alpha Innotech). Multiple exposures of each blot were routinely taken, and the exposure that had specific protein bands within the linear range in optical density was used for densitometry.
Quantitative western blot analyses were based on three or more independent experiments after densitometry tracing of specific protein bands using the Scion Image software (version 18.104.22.168, Scion Corporation). The optical densities of the protein bands in equal area of space were determined after subtracting the background per individual lane. In order to analyze the results across different experiments, the optical density levels were then normalized to γ-tubulin expressions in the respective western blot. The normalized density units were then analyzed by one-tail or two-tail t-Tests (more stringent) for two samples assuming unequal variance using the EXCEL data analysis tool (Microsoft Corporation). A p value of 0.05 or less was considered to be statistically significant.
Cell membrane, cytosolic and nuclear fractions
The post-nuclear membrane fraction was isolated as described . Briefly, after transfection of HEK293 cells for 40 hours, or after infection of primary neuronal cultures for 15 hours, the medium was withdrawn, and cells were harvested in ice-cold PBS, washed once, and homogenized by shearing through a 22-ga needle in buffer HS (250 mM sucrose, 150 mM NaCl, 10 mM Tris-HCl, and 5 mM EDTA, pH 7.4) supplemented with a mixture of protease inhibitors (Sigma). All subsequent steps were carried out on ice unless indicated otherwise. The crude nuclear fraction was saved after the samples were centrifuged at 1500 × g for 10 min and resuspended in buffer HD (10 mM Tris-HCl, pH 7.4, 150 mM NaCl, 1% SDS, and 5 mM EDTA) with protease inhibitors. Membrane fractions were collected from the postnuclear supernatants by centrifugation for 20 min at 14,000 × g and resuspended in buffer HD with protease inhibitors. Proteins in the supernatant (cytosolic fraction) were precipitated with 20% trichloroacetic acid. The precipitated proteins were washed with 95% ethanol. Protein pellets were resuspended in 1% Triton X-100 containing protease inhibitor mix (1:250). Equal amount of proteins from membrane, cytosolic or nuclear fractions were resolved by SDS-PAGE, transferred to nitrocellulose membrane, and analyzed for β-catenin by western blot analyses.
Dual luciferase assays
HEK293 cells were transfected with pGL3-OT or pGL-OF (improved versions of pTOPflash and pFOPflash, respectively)  and APP or a mutant APP construct. Renella luciferase reporter (CMV-PRL, Promega) was included in each sample to normalize transfection efficiency. The positive control was prepared from cells transfected with β-catenin . Cells were harvested at 40 h after transfection and dual luciferase assays were performed as described in the manufacturer's protocol (Promega). Luciferase activity was measured by a dual-injector microplate luminometer (Turner Biosystems) using Veritas program.
Primary neurons were fixed with 4% paraformaldehyde for 40 m at room temperature. Cells were then washed with PBS, blocked with 3% normal goat serum, and stained with rabbit anti-β-catenin (Sigma) for 2 h at room temperature. Cells were then washed and incubated with Alexa Fluor 488-conjugated goat anti-rabbit for 1 h (Molecular Probe). Counterstaining with DAPI was performed in some cells by incubating for 2 m with DAPI (20 μg/ml). After 4× washes in PBS, cells were mounted in 90% glycerol. Negative controls were without primary antibodies. The specificity of the anti-β-catenin antibody was also demonstrated in western blots. Confocal images were taken under a 63× objective with a Nikon D-Eclipse C1 confocal microscope through z-series at the same settings. Individual z-sections and composite images were further grouped in Photoshop (version 6.0, Adobe).
APP knockout animals and immunofluorescence labelling
APP knockout animals were raised and genotyped as described before (n = 4; 3 were 8 months old and 1 was 18 months old) and WT controls (n = 4; 3 were 8.5 months old and one was 7 months old) . Brain sections (6 μm thick) were pre-incubated with 2N HCl for 30 m, washed 6×, blocked with 3% normal goat serum, and incubated overnight in primary antibodies. The sections were then washed 3×, and incubated in secondary antibodies for 1 h before incubation in DAPI solution for 2 m. Sections were washed and mounted in 90% glycerol. Images were obtained at the same settings with a Nikon Eclipse 600 fluorescence microscope and CoolSnap digital camera using MetaVue software (version 6.2r2, Molecular Devices Corporation). The pixel density of the CA1 pyramidal cells in the cell body layer were sampled using the MetaVue software. The mean value of pixel density was calculated and compared by two-tailed t-Test assuming unequal variance (Excel, Microsoft).
APP downregulates β-catenin in primary neurons
APP facilitates β-catenin degradation by increasing β-catenin phosphorylation at S33/37/T41
Downregulating endogenous APP significantly inhibits β-catenin phosphorylation at S33/37/T41 but not at S45
APP-expression decreases β-catenin in membrane and cytosolic fractions without affecting nuclear β-catenin
In contrast to membrane and cytosolic β-catenin, nuclear β-catenin did not appear to change upon expression of wild-type or FAD APP (Fig. 4A). To obtain further support for the fractionation experiments, we then tested the nuclear function of β-catenin using luciferase reporter assays. HEK293 cells were transfected with wild-type or FAD APP, along with the TCF luciferase reporter plasmid (pGL3-OT). None of the APP constructs consistently decreased pGL3-OT luciferase reporter activity. Controls included cotransfection of a mutant TCF luciferase reporter (pGL3-OF) with APP, and cotransfection of pGL3-OT with pcDNA3 (data not shown). A positive control was prepared from cells transfected with a β-catenin expression construct and the pGL3-OT plasmid. Together, these data suggest that APP may not affect β-catenin transcriptional activity.
To complement the above experiments, confocal microscopy was used to assess β-catenin levels and cellular locations in primary neurons. Primary neurons expressing APP or LacZ (control) were fixed and labelled with the rabbit anti-β-catenin antibody and the Alexa fluor 488 goat anti-rabbit antibody. Representative z-sections of the same cells are presented in Fig. 4B. The z-sections show abundant β-catenin present near or at the plasma membrane. More β-catenin seemed to localize in the basal-lateral than apical regions, and APP expression did not seem to affect β-catenin localization compared to the LacZ control. The z-series (Fig. 4B) and the composite images (Fig. 4C) also revealed that β-catenin fluorescence intensity decreased dramatically in APP-expressing neurons compared to the LacZ control, further supporting the data obtained by fractionation assays.
β-Catenin is significantly increased in CA1 pyramidal cells from APP knockout animals
In this report, we provide strong evidence that APP mediates β-catenin downregulation. We demonstrate that APP downregulates β-catenin levels in primary neurons by facilitating specific phosphorylation of S33/37/T41 residues in β-catenin. APP expression is inversely correlated with the levels of total β-catenin. Corroborating data were obtained using APP siRNAs: suppression of APP by siRNAs increased steady-state β-catenin levels and reduced the levels of S33/37/T41 phosphorylation in neurons. We further show that β-catenin accumulates in hippocampal pyramidal cells in APP knockout animals. Together, these data establish that APP is physiologically important in maintaining β-catenin homeostasis, which is likely critical for neuronal survival and function by preventing aberrant cell cycle reaction.
We show that familial AD mutants of APP induce similar β-catenin degradation, suggesting that familial AD mutants retain similar functions. Our method might not be sensitive enough to detect the degree of differences in β-catenin downregulation by these APP mutants upon acute expression in cell cultures. Long-term effects of APP mutants on β-catenin expression could be analyzed in transgenic animals. In primary neurons, APP-induced β-catenin downregulation did not appear to affect nuclear β-catenin or its transcriptional activity. However, β-catenin accumulation in CA1 pyramidal neurons from APP knockout animals does appear to affect transcriptional activity, judging from the increases found in cyclin D1 protein levels in these same neurons. These observations illustrate the limitations of luciferase reporter assays in primary neurons; they also suggest that basal levels of β-catenin are necessary for neuronal function, but that these do not necessarily affect β-catenin-mediated transcription.
Several questions remain to be answered, such as whether APP processing products, such as secreted APP, or Aβ, mediate the effect of APP on β-catenin degradation. The effect of APP on β-catenin phosphorylation could also reflect the interaction between APP and APP-BP1. APP-BP1 activates neddylation and increases ubiquitinylation by the Cullin-based E3 ligase. Ubiquitinylation of β-catenin may be facilitated by the interaction between APP and APP-BP1, which is not unidirectional as indicated by the studies in Drosophila . We have recently shown that one function of APP-BP1 is to downregulate Aβ1–42 in primary neurons . Aβ1–42 also appears to downregulate β-catenin (YC unpublished observations). However, it remains to be determined whether APP and Aβ1–42 modulate β-catenin degradation through the same pathways.
The roles of APP and PS1 on β-catenin phosphorylation may be independent of each other. We show that APP facilitates β-catenin phosphorylation at S33/37/T41 residues. Others have shown that PS1 expression can enhance phosphorylation of β-catenin at S45, which may prime the phosphorylation of S33/37/T41  and facilitate membrane β-catenin delivery and degradation [17, 18]. The ultimate effect of PS1 on β-catenin degradation remains controversial. Some studies have shown destabilization of β-catenin by wild-type PS1 but inactivity of the FAD-mutant forms of PS1 [20, 22]; others have shown the opposite . Serban et al.  argued that the ultimate outcome rests on the inherent levels of E-cadherin. Our new findings suggest that PS1 and APP may impinge on different components in the β-catenin degradation pathway, but the underlying mechanism needs to be further investigated.
Our new findings not only support a critical role for APP in maintaining neuronal differentiation but also support a role for APP in synaptic dynamics due to the multifaceted functions of β-catenin [40, 41]. Cell cycle events are widely documented in post-mortem AD brain tissues . In several AD cases which we have examined, almost all hippocampal neurons show signs of cell cycle entry as indicated by the cytoplasmic translocation of Nedd8 . This cell cycle deregulation and synaptic dysfunction may well be related . Our new findings suggest a dysfunction of APP in maintaining neuronal differentiation in AD neurons. However, levels of APP itself must be regulated, as high levels of APP could induce neuronal death [7, 44]; our new evidence suggest that low levels of APP may be equally detrimental to neurons due to β-catenin accumulation. We observed a large amount of β-catenin in the plasma membranes of primary neurons (Fig. 4), in accord with findings reported in Drosophila . Membrane β-catenin is known to play a role in dendritic remodeling in mature neurons . Synaptic dynamics may involve changes in the interaction of β-catenin with cytosolic or membrane proteins such as with E-cadherin. These considerations, taken together, implicate APP as a critical factor in neuronal function that warrants further investigation.
In summary, this report documents a function of APP in β-catenin downregulation in vivo and in vitro. These findings open new avenues for research involving the role of APP processing in β-catenin downregulation. Future studies may also determine whether excessive APP expression contributes to AD pathogenesis involving abnormal β-catenin phosphorylation and degradation in transgenic animals.
List of abbreviations
amyloid precursor protein
day in vitro
small interfering RNA
small hairpin RNA.
We thank Dr. Hui Zheng for providing APP KO mouse brains, Dr. Bert Vogelstein and Kenneth W. Kinzler for providing pGL3-OT and pGL3-OF plasmids, and Dr. David Kimelman for the xenopus β-catenin expression vector. We thank Dr. Steven Barger for critical reading of the manuscript, Dr. W. Sue T. Griffin for helpful discussions, Sue Woodward for technical assistance, and Dr. Edgar Garcia-Rill for access to their confocal microscope. Confocal microscopy was supported by the Center for Translational Neuroscience award RR020146a (E. Garcia-Rill).
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