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The Journal of Neuroscience, May 31, 2006, 26(22):6011-6018; doi:10.1523/JNEUROSCI.1189-06.2006

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Neurobiology of Disease
Different Conformations of Amyloid Induce Neurotoxicity by Distinct Mechanisms in Human Cortical Neurons

Atul Deshpande,¹ Erene Mina,² Charles Glabe,^2,3 and Jorge Busciglio^1,3

Departments of ¹Neurobiology and Behavior and ²Molecular Biology and Biochemistry, and ³Institute for Brain Aging and Dementia, University of California, Irvine, Irvine, California 92697

	Abstract

Top Abstract Introduction Materials and Methods Results Discussion References

 
Characterization of soluble oligomeric amyloid (A) species in the brains of Alzheimer's disease (AD) patients and transgenic models has raised the possibility that different conformations of A may contribute to AD pathology via different mechanisms. To characterize the toxic effect of different A conformations, we tested side by side the effect of well characterized A oligomers (AOs), A-derived diffusible ligands (ADDLs), and fibrillar A (Af) preparations in human cortical neurons (HCNs). Both AOs and ADDLs bind rapidly and with high affinity to synaptic contacts and cellular membranes. AOs (5 µM) induced rapid and massive neuronal death. Calcium influx accelerated, but was not required for, AO toxicity. AOs elicited a stereotyped succession of cellular changes consistent with the activation of a mitochondrial death apoptotic pathway. At low concentrations AOs caused chronic and subtler mitochondrial alterations but minimal cell death. ADDLs induced similar toxic changes as AOs but on a fivefold longer time scale. Higher concentrations of Af and longer incubation times were required to produce widespread neuritic dystrophy but modest HCN cell death. Thus various A species may play relevant roles in AD, causing neurotoxicity by distinct non-overlapping mechanisms affecting neuronal function and viability over multiple time courses.

Key words: amyloid ; oligomers; Alzheimer's disease; apoptosis; mitochondria; synapses

	Introduction

Top Abstract Introduction Materials and Methods Results Discussion References

 
Typical neuropathological features of Alzheimer's disease (AD) include the presence of senile plaques, neurofibrillary tangles, and neuronal loss in the cortex and hippocampal formation of affected individuals. Senile plaques are composed mainly of amyloid (A) peptide in its fibrillar form. Fibrillar A (Af) triggers a variety of pathological changes including tau hyperphosphorylation, leading to neuronal dysfunction and degeneration (Busciglio et al., 1992, 1995; Pike et al., 1992; Geula et al., 1998). In culture, the chronic exposure of neurons to Af induces aberrant activation of adhesion signaling pathways, neuritic dystrophy, and synaptic loss (Grace et al., 2002; Grace et al., 2003). In vivo imaging in transgenic models show neuritic dystrophy and distortion in direct apposition with Af deposits (Tsai et al., 2004; Spires et al., 2005), which cause alterations in neocortical synaptic responses (Stern et al., 2004). Fibrillization of A is preceded by multiple conformational changes including trimer, pentamer, or higher molecular weight complex formation, also known as A-derived diffusible ligands (ADDLs) (Lambert et al., 1998), oligomers composed of 15–20 monomers (AOs) (Kayed et al., 2003), protofibrils (string of oligomers) (Nguyen and Hall, 2004), and dodecameric oligomers A*56 (Lesné et al., 2006). These intermediate A species are designated collectively as "soluble A" (Glabe, 2004). Soluble A species are found in cerebrospinal fluid of AD patients (Kuo et al., 1996; Georganopoulou et al., 2005), can be neurotoxic at low concentrations, and induce inhibition of long-term potentiation and cognitive dysfunction in rodents (Lambert et al., 1998; Hartley et al., 1999; Dahlgren et al., 2002; Walsh et al., 2002b; Lesné et al., 2006). Most relevant, the brain levels of soluble A species appear to correlate better than density of plaque deposition with severity of cognitive impairment (Lue et al., 1999; Naslund et al., 2000). In this regard, oligomers derived from different amyloidogenic proteins have been proposed as primary toxic species in several neurodegenerative diseases, including prion in spongiform encephalopathies, -synuclein in Parkinson's disease, and polyglutamine in Huntington's disease (Lashuel et al., 2002b; Caughey and Lansbury, 2003; Kayed et al., 2003; Sanchez et al., 2003). Oligomer toxicity appears to be related to a common conformational state, because various oligomers react with the conformation-dependent antibody A11 and oligomeric forms of nondisease-related proteins and peptides are equally toxic (Bucciantini et al., 2002; Kayed et al., 2003, 2004; Demuro et al., 2005). These results raise the possibility that different conformations of A, including soluble and fibrillar A species, may contribute to AD pathology via different mechanisms. To address this issue, we tested side by side the effect of well characterized AO, ADDL, and Af preparations on neuronal function and viability. We used cultured human cortical neurons (HCNs), one of the principal cell types affected in AD. The results show that A species cause neurotoxicity by multiple mechanisms, affecting neuronal function and viability at various concentrations and over different time courses. Thus several A species may play relevant roles in AD by exerting distinct deleterious effects on neuronal cells during the disease process.

	Materials and Methods

Top Abstract Introduction Materials and Methods Results Discussion References

 
Neuronal cultures. Neuronal cultures were established from 16-to 21-week-old human fetal brain tissue as described (Busciglio et al., 2002; Pelsman et al., 2003). The protocols for tissue procurement complied with federal and institutional guidelines. Briefly, the cells were dissociated into single-cell suspensions by incubation with 0.25% trypsin/ PBS at 37°C for 30 min and mechanically dissociated by using a fire-polished glass Pasteur pipette. Cells were plated at a density of 20,000 cells/cm² in 24- or 96-well plates and 35 and 60 mm dishes. At 2 h after plating the medium was changed to Neurobasal medium plus N2 and B27 supplements (Invitrogen, Grand Island, NY). Partial medium changes (50%) were performed every 5 d. For low calcium experiments, after the initial 5 d, 11 consecutive daily medium changes were performed with calcium-free DMEM plus N2 and B27 supplements to reach a 50 nM calcium concentration in the culture medium. Control cultures received similar medium changes, but normal calcium levels were preserved in the culture. Alternatively, magnesium concentration was increased to 400 µM while calcium was decreased simultaneously to 50 nm on 15 d in vitro (15 DIV). Both protocols worked well, yielding equivalent results.

A treatments. AO preparations have been characterized in previous studies (Kayed et al., 2003). A detailed protocol for the preparation of AOs is included by Demuro and colleagues (2005). AO preparations have an approximate molecular mass of 90 kDa and contain very little material of lower molecular mass; the ultrastructural analysis indicates that they are composed of spherical vesicles with diameters of 2–5 nm (Demuro et al., 2005). Comprehensive descriptions of ADDL preparations also have been published previously (Lambert et al., 1998; Chromy et al., 2003). ADDL solutions have a heterogeneous composition and show a major component migrating at 17 kDa in addition to several minor faster and slower migrating bands. The molecular weights of ADDLs formed in vitro are consistent with A trimer, tetramer, pentamer, and higher molecular weights up to 24-mer (Lambert et al., 1998; Chromy et al., 2003). Fibrillar and oligomeric A_1–42 was prepared as described (Demuro et al., 2005). ADDLs were prepared with A_1–42 peptide provided by Dr. W. Klein (Northwestern University, Evanston, IL) and followed the standardized protocol (Lambert et al., 1998; Lacor et al., 2004). For some experiments a kit was used to label Af with Alexa Fluor 350 (Invitrogen Molecular Probes, Carlsbad, CA), following the manufacturer's instructions. A preparations were added to the cultures at 18 DIV, and viability was assessed at the indicated time points.

Immunofluorescence. Neurons were fixed in 4% paraformaldehyde and 0.12 M sucrose in PBS for 30 min at 37°C, permeabilized with 0.2% Triton X-100 in PBS, and blocked for 1 h in 5% bovine serum albumin/PBS. Then the cultures were incubated with mouse anti-synaptophysin (1:500; Calbiochem, La Jolla, CA), rabbit anti-tau (1:1000; Dako, Carpinteria, CA), anti-oligomer A11 (1:2500) (Kayed et al., 2003), anti-A 6E10 (1:1000; Signet, Dedham, MA), mouse anti-PSD-95 (1:1000), a gift from Dr. Matthew Rasband (University of Connecticut Health Center, Farmington, CT), mouse anti-cytochrome c (cyt c; 1:600; BD Transduction Laboratories, San Diego, CA), or rabbit anti-apoptosis-inducing factor (AIF; 1:500; Chemicon, Temecula, CA) for 24 h at 4°C, followed by incubation in fluorescent-conjugated secondary antibodies (Alexa, Invitrogen Molecular Probes). Triple labeling was performed by sequential incubation with the appropriate antibodies. Competition with antigenic peptide, use of non-immune IgG instead of primary antibody, or omission of primary antibody resulted in complete elimination of specific labeling. An Axiovert 200 inverted microscope (Zeiss, Jena, Germany) was used for specimen examination and imaging. Fluorescent images were captured with a digital camera (Zeiss) at a final magnification of 630x and processed by using AxioVision (Zeiss). To assess colocalization of synaptic markers, we used an apotome device (Zeiss) for z-sectioning. To quantify the frequency of colocalization of fluorescent signals, we captured at least 20 fields per section of each individual case at a final magnification of 630x and analyzed them with AxioVision software (Zeiss). To avoid bias, we performed colocalization assessments in coded preparations. To confirm triple colocalization of fluorescent markers, we used TetraSpec beads (Invitrogen Molecular Probes) as a positive control. Each 500 nm bead is labeled with four different fluorophores, enabling us to correct for potential plane shifts associated with each individual fluorescent filter (TetraSpeck Fluorescent Microspheres Sampler kit; Invitrogen Molecular Probes).

Time-lapse imaging. HCNs grown on 35 mm glass-bottom culture dishes treated with A preparations or vehicle alone were placed in a temperature- and CO₂-controlled incubator chamber mounted on the microscope stage. Time-lapse images that used differential interference contrast (DIC) optics were taken every 30 min for 24 h at 400x final magnification. During experiments the temperature was maintained at 37°C, and the CO₂ concentration was held at 5%. For quantitative image analysis, random microscopic fields were selected (at least 15 microscopic fields per culture dish in at least triplicate dishes). Microscopic fields were selected randomly, with care taken to select a similar number of fields per quadrant of the 12 mm glass area (seven to eight fields/quadrant) of glass-bottom 35 mm culture dishes. The culture dish remained in the culture chamber on the stage of the automated microscope at all times during the experiments. Selection of fields for analysis was performed by using the "mark and find" function immediately before the initiation of the treatments. Then the image acquisition software automatically returned to the selected fields to capture images at each predetermined time point. Once the experiment was finished, the image analysis software marked each scored object (e.g., condensed nucleus) and then added up the number of scored objects per field for each time point, ruling out the possibility of scoring the same object more than once.

Cell death and mitochondrial assays. Cell death was assessed by quantifying lactate dehydrogenase release to the cultured medium with the use of a commercial kit (CytoTox 96; Promega, Madison, WI) and by counting the number of condensed nuclei per microscopic field at 400x final magnification. At least 10 fields per culture in triplicate cultures were analyzed per individual experiment. Caspase 3 and 7 activities were quantified by using the Caspase-Glo 3/7 kit (Promega). Mitochondrial oxidoreductase activity was determined by analyzing the ability of mitochondria to convert a tetrazolium compound to formazan. The reagent 3-[4,5-dimethylthiazol-2-yl]-5-[3-carboxymethoxyphenyl]-2-[4-sulfophenyl]-²H-tetrazolium (MTS) is reduced to formazan by mitochondrial succinate dehydrogenase in complex II (succinate/ubiquinone oxidoreductase complex) and possibly other complexes of the electron transport chain (CellTiter 96 AQ_ueous; Promega) (Busciglio et al., 2002). ATP level was quantified by using a luminescence assay (CellTiter Glo, Promega). Mitochondrial membrane potential (MMP) was determined by using the fluorescent probe JC1 as described previously (Busciglio et al., 2002). Briefly, HCNs cultured in black-wall clear bottom plates were labeled with JC1 (1 µg/ml) at 37°C for 20 min and washed twice with medium. JC1 fluorescence was measured on a 96-well fluorescence reader (Gemini Spectra XPS, Molecular Devices, Union City, CA), and relative changes in MMP were assessed as the change in JC1 590/525 fluorescence ratio. Similar studies also were performed with two other commonly used mitochondrial and cell membrane potential indicators: tetramethylrhodamine ethyl ester (TMRE) at 100 nM for 10 min and bis-(1,3-dibutylbarbituric acid)-trimethine oxonol [DiBAC₄(3)] at 100 nM for 20 min.

Statistical analysis. All experiments were repeated at least three times in cultures derived from at least three different fetal specimens. Each individual experiment was performed in triplicate cultures. Data were analyzed by unpaired Student's t test and expressed as the mean ± SEM. Significance was assessed at p < 0.05. All reported results correspond to single representative experiments.

	Results

Top Abstract Introduction Materials and Methods Results Discussion References

 
Synaptic localization of AOs and ADDLs
Initial tests were performed to validate the experimental model and the effectiveness of A preparations to induce cellular responses. By 15–20 DIV the HCN cultures developed a dense network of neuronal processes, compartmentalized MAP2 (mitogen-activated protein 2) and tau in somatodendritic and axonal compartments, respectively, and established numerous active synapses (supplemental Fig. 1, available at www.jneurosci.org as supplemental material) (Kerkovich et al., 1999). To study the effects that soluble and fibrillar A species have in differentiated neurons, we initiated treatments at 18 DIV. Previous work has shown a very specific synaptic targeting of ADDLs in rat hippocampal neurons in culture (Lacor et al., 2004). To determine whether AOs also were localized to synaptic sites, we fixed HCN cultures treated with 5 µM AOs at 30 min and 1 h after initiation of the incubation, and we performed triple immunofluorescence with anti-synaptophysin, anti-postsynaptic density-95 (anti-PSD-95), and anti-oligomer (A11) or anti-A (6E10) antibodies. Synapses were defined by the colocalization of the presynaptic and postsynaptic markers synaptophysin and PSD-95 (supplemental Fig. 1, available at www.jneurosci.org as supplemental material). We found a clear time-dependent increase in the number of AOs bound to cells in cultures fixed at 30 min and 1 h (data not shown). Multiple fluorescence labeling demonstrated a striking colocalization of oligomers with presynaptic and postsynaptic markers (Fig. 1A). Approximately 43 ± 13% of synapses labeled positive for AOs with the anti-oligomeric specific antibody A11 (Fig. 1B). We also investigated the localization of ADDLs (5 µM) in HCNs at similar time points. We found that ADDLs have a slightly higher preference for synaptic localization (54 ± 11%) than AOs (Fig. 1B). Similar results were obtained by using anti-A 6E10 antibody (data not shown). Thus both AOs and ADDLs bind rapidly and with remarkable specificity to synaptic sites in HCN cultures.

View larger version (37K): [in this window] [in a new window]   Figure 1. AOs colocalize with synaptic markers in HCNs. A, Triple immunofluorescence of 18 DIV HCNs with AOs (A11, green; 1:2500), anti-PSD-95 (red; 1:1000), and anti-synaptophysin (blue; 1:500). Cultures were incubated with 5 µM AOs for 1 h before fixation. The overlay image shows the colocalization of the three antibodies. Triple colocalization is observed as light yellow fluorescent spots (arrows). Scale bar, 5 µm. B, Quantification of the frequency of colocalization of AOs and ADDLs (antibody A11) with the synaptic markers PSD-95 and synaptophysin (Syn.). Error bars indicate the mean ± SEM.

 
A-soluble species cause a fast and massive toxic effect, whereas A fibrils induce progressive dystrophy and modest cell death in HCNs
Earlier experiments characterized the dystrophic effect of Af on rat cortical and hippocampal neurons (Pike et al., 1992; Grace et al., 2002; Grace and Busciglio, 2003). A similar dystrophic-inducing effect of Af was observed on HCNs. Chronic exposure of HCNs to 20 µM Af for 10 d induced progressive dystrophy, including wavy shapes, sharp angles, tortuosity, and formation of loops in neuronal processes (Fig. 2B,C). No such changes were observed in control neurons treated with vehicle (Fig. 2A). Despite these dramatic changes in neuronal morphology and consistent with previous results in rat cortical neurons (Grace et al., 2002), only modest cell death (20 ± 7%) was observed after 10 d of treatment with Af. In sharp contrast, 5 µM of AOs induced rapid and extensive cell death in HCNs (Fig. 2D–G) (see also the supplemental movie, available at www.jneurosci.org as supplemental material). HCNs treated with AOs showed rapid changes in morphology as compared with those treated with Af. In the presence of AOs neuritic retraction was observed as early as 3 h after initiation of the treatment, followed by progressive apoptotic features, including disintegration of neuronal processes, swelling of cell bodies, and nuclear condensation (Fig. 2E,F). The supplemental movie (available at www.jneurosci.org as supplemental material) contains a complete time-lapse sequence starting at time point 0 (Fig. 1D) and finishing 24 h later (Fig. 1E). By 12 h 30 ± 8% of the neurons were lost, and by 24 h 73 ± 5% of the cells were dead (Fig. 2H). The effect of AOs was dose-dependent. Incubation with 2 µM AOs required 96 h to induce massive death, and incremental concentrations (5, 10, and 20 µM) showed faster and higher toxic rates (Fig. 2H). The toxic effect was reduced markedly by the preincubation of AO preparations with anti-oligomer A11 or anti-A 6E10 antibodies before their addition to the cultures or by simultaneous addition of A and A11 antibodies to the cultures (data not shown).

View larger version (96K): [in this window] [in a new window]   Figure 2. AOs cause rapid and massive neuronal death. Shown is double immunofluorescence of 18 DIV HCNs with anti-tau (red; 1:500) and anti-A (blue). A, Neuronal processes in vehicle-treated HCNs exhibit considerable development and a normal, smooth appearance (Ctrl). B, After 10 d of treatment with 20 µM Af, neuronal processes display aberrant morphologies, including tortuosity and irregular neuritic caliber. C, Combined DIC/fluorescence at higher magnification illustrates a neuronal process exhibiting loops and sharp turns close to Af deposits (blue). D–F, DIC images of living HCN cultures treated with 5 µM AOs. Immediately after AO addition, the culture exhibits a normal appearance (D); after 24 h, extensive cell death is indicated by retraction and disintegration of processes and nuclear condensation (E, arrows). At higher magnification the beading and disintegration of neuronal processes are observed clearly (F, arrows). The supplemental movie (available at www.jneurosci.org as supplemental material) contains a complete time-lapse sequence of this experiment. Scale bars, 20 µm. G, Quantification of condensed nuclei/field over the 24 h period of AO treatment. The graph illustrates one representative field. At least 20 different fields were analyzed with similar results. H, Bar graph illustrating the increase in condensed nuclei in HCN cultures treated with increasing concentrations of AOs. The number of condensed nuclei was scored at the indicated time points. Similar results were obtained in five independent experiments. Error bars indicate the mean ± SEM.

 
To characterize the death process further, we analyzed three parameters associated with apoptosis and loss of cell viability after 24 h of AO treatment (5 µM): mitochondrial metabolic activity, caspase activation, and lactate dehydrogenase (LDH) release. Mitochondrial activity was studied by using an oxidoreductase assay, which measures the amount of formazan salt converted to a soluble-colored product by mitochondria (MTS assay). By 24 h a significant drop of 61 ± 11% in mitochondrial oxidoreductase activity was observed in HCNs treated with AOs (Fig. 3D). We also analyzed the levels of activated caspases 3 and 7, which are critical mediators of the execution phase of apoptosis (Earnshaw et al., 1999; Slee et al., 1999; Fan et al., 2005). We found a 224 ± 24% increase in caspase activity as compared with control or Af-treated cells (Fig. 3E). Similarly, there was a major increase in LDH level (257 ± 18%) in the medium of AO-treated cultures after 24 h (Fig. 3F), indicating massive cell death.

View larger version (35K): [in this window] [in a new window]   Figure 3. AO toxic effect under normal and low extracellular calcium. A, D, Mitochondrial oxidoreductase activity at 12 h (A) and 24 h (D). B, E, Caspase 3 and 7 activation at 12 h (B) and 24 h (E). C, F, LDH levels in the culture medium at 12 h (C) and 24 h (F). Under normal culture conditions, these three parameters are significantly different from controls (Ctrl) after 12 h of AO treatment (A–C). Under low calcium conditions, no significant differences in any of these parameters are observed between Ctrl and AO-treated cultures at 12 h (A–C). By 24 h, there is a significant enhancement of neurotoxic parameters in AO-treated cultures under both normal and low calcium conditions (D–F). Similar results were obtained in four independent experiments. Values are expressed as the mean ± SEM by unpaired Student's t test; *p < 0.05; **p < 0.01.

 
At a similar concentration the ADDLs induced neurotoxicity on a much slower time course. Only after 5–7 d of continuous ADDL exposure did changes in mitochondrial oxidoreductase activity reach a similar level to that of AO-treated cells for 24 h. After 7 d of ADDL treatment the caspase activation was elevated to a lesser but significant extent when compared with that of AO-treated cultures for 24 h. Consistent with these results, the LDH level was elevated only slightly by 7–8 d, indicating only moderate cell death in ADDL-treated cells (data not shown). Thus AOs induced rapid apoptotic changes on HCNs, whereas similar concentrations of ADDLs resulted in comparable changes but on a markedly slower time course. No significant modifications in mitochondrial activity, caspase activation, or LDH release were present in HCNs treated with Af for 24 h (data not shown). Thus soluble (AOs and ADDLs), but not fibrillar, A species are associated with HCN apoptotic cell death in culture.

Previous studies indicate that A-soluble species are toxic at very low concentrations in different experimental paradigms (Hartley et al., 1999; Walsh et al., 22217; Kayed et al., 2003; Demuro et al., 2005). To assess the effect of A species at lower doses, we analyzed the effect of AOs at 10 nm, 100 nm, and 1 µM. At 1 µM and 100 nm the AOs decreased MMP significantly within 6 h (35.7 ± 7 and 54.2 ± 13%, respectively) (supplemental Fig. 2, available at www.jneurosci.org as supplemental material). At 10 nM AOs the MMP did not change as compared with control cells. At 1 µM and 100 nm AOs the ATP levels dropped to 50%, in both cases by day 3 (supplemental Fig. 2, available at www.jneurosci.org as supplemental material). LDH levels in the supernatant increased by only 10% in HCNs treated with 1 µM and 100 nm AOs at the end of day 3 (data not shown). These results indicate that, although low concentrations of AOs do not cause significant neuronal loss, they induce early and chronic alterations in mitochondrial function that may impact overall neuronal homeostasis.

Calcium influx accelerates, but is not essential for, AO-induced neurotoxicity
Recent experiments demonstrated that AOs induce a fast calcium influx in neuroblastoma cells (Demuro et al., 2005), and numerous studies have implicated increased intracellular calcium as a central event in apoptotic processes in various cell types (Duchen, 2000; Polster and Fiskum, 2004). To establish the role of calcium in AO neurotoxicity, we grew HCNs under normal or low calcium concentration conditions (see Materials and Methods) and treated them with 5 µM AOs. Data collected at 12 h indicated that, in the presence of normal calcium levels, there was a significant decrease of 41 ± 25% in mitochondrial oxidoreductase activity (Fig. 3A), a 40 ± 11% increase in caspase activity (Fig. 3B), and 26 ± 6% higher LDH levels in the culture medium (Fig. 3C). These changes were not observed in neurons treated for 12 h with AOs under low calcium conditions (Fig. 3A–C). However, by 24 h the levels of oxidoreductase activity, caspase activation, and LDH release were similar to those in HCN cultures exposed to AOs in the presence of calcium (Fig. 3A–C). These results suggest that, although calcium influx can accelerate AO toxicity markedly, it is not an absolute requirement for the toxic effect of soluble A species. There were no differences in the dystrophic effect induced by Af in normal and low calcium conditions (data not shown).

AOs activate a mitochondrial death pathway
In many paradigms of apoptosis a mitochondrial death pathway is activated by signaling molecules recruited to mitochondria, leading to a rapid drop of MMP and ATP levels, opening of the mitochondrial transition pore (MTP), translocation of cyt c and AIF from the mitochondrial matrix to the cytoplasm, and activation of caspases in charge of the "execution" phase of the death process (Johnstone et al., 2002; Danial and Korsmeyer, 2004; Helguera et al., 2005). To delineate further the chain of events triggered by A species, we analyzed mitochondrial changes at early time points after A treatment, before the occurrence of massive cell death. Mitochondrial membrane potential, measured as the emission ratio of red over green fluorescence (590/525 nm) of the fluorescent probe JC-1, dropped drastically within the first 2 h of exposure to AOs (89 ± 15%) (Fig. 4A). Comparable results were observed by using the fluorescent probes TMRE and DiBAC₄(3), two other commonly used mitochondrial and cell membrane potential indicators, respectively (data not shown). Similarly, ATP levels dropped 70 ± 10% by 2 h and decreased steadily thereafter (Fig. 4B). Caspase activation and LDH release increased 35 ± 6 and 23 ± 8%, respectively, by 8 h (Fig. 4C,D). Treatment with 5 µM ADDLs decreased MMP and ATP levels progressively but to a lesser extent as compared with AOs at similar concentrations (data not shown). Changes in mitochondrial membrane potential were observed only after 5 d of treatment with 20 µM Af, because it decreased 34 ± 4% as compared with controls, whereas ATP levels decreased 33 ± 9%, indicating that dystrophic neurons also exhibit mitochondrial impairment.

View larger version (25K): [in this window] [in a new window]   Figure 4. AOs induce rapid mitochondrial alterations in HCNs. A–D, MMP, ATP levels, caspase activity, and LDH release were quantified in control (Ctrl) and AO-treated cultures (5 µM) at the indicated time points. Significant changes in MMP and ATP levels can be observed in AO-treated cultures within 2 h of treatment (A, B). Significant changes in caspase activity and LDH release are detected by 8 h (C, D). Values are expressed as the mean ± SEM by unpaired Student's t test; *p < 0.05; **p < 0.01. Similar results were obtained in four independent experiments.

 
Mitochondrial release of cyt c and AIF is a direct consequence of increased permeability of the mitochondrial membrane mediated by the mitochondrial permeability transition pore (Danial and Korsmeyer, 2004). Immunofluorescence analysis revealed that both cyt c and AIF showed diffuse cytoplasmic localization in cell bodies and processes of HCNs treated with AOs for 8 h, which were devoid of obvious degenerative morphology (Fig. 5). In contrast, discrete labeling and restricted mitochondrial localization of cyt c and AIF were observed in cell bodies and processes of HCNs treated with vehicle (Fig. 5, Ctrl). Similarly, HCNs treated with ADDLs for 96 h showed diffuse cytoplasmic localization of cyt c and AIF (Fig. 5). Thus early mitochondrial changes consistent with activation of a mitochondrial death pathway are present early on during soluble A toxicity.

View larger version (82K): [in this window] [in a new window]   Figure 5. Soluble AOs induce translocation of cyt c and AIF from mitochondria to the cytoplasmic compartment. Shown is immunofluorescence of HCNs treated with vehicle (Control), AOs, or ADDLs for the indicated times. Control cultures incubated with vehicle for 96 h exhibit mitochondrial localization of cyt c and AIF in cell bodies and processes (green fluorescence). In contrast, AO- and ADDL-treated cultures exhibit diffuse cyt c and AIF localization in both cell bodies and neuronal processes (green fluorescence). The bottom panels are higher magnifications of the boxed areas. Scale bars, 10 µm. Neurons were double-labeled with the neuronal-specific marker anti-tubulin Class III (red fluorescence). Nuclei were counterstained with Hoechst (blue fluorescence).

 

	Discussion

Top Abstract Introduction Materials and Methods Results Discussion References

 
To understand the pathophysiology of AD, it is critical to elucidate the role of A and its different conformations in the disease process. We used primary HCNs, the target cells in AD, as an experimental paradigm to show that Af, AO, and ADDL preparations affect neuronal function and viability by distinct toxic mechanisms, suggesting that A neurotoxicity in AD is a complex and multifaceted phenomenon.

The presence of Af in the AD brain is well established as the major component of senile plaques. Previous work demonstrates that Af is toxic to primary neurons (Busciglio et al., 1992, 1995; Pike et al., 1992; Geula et al., 1998). Chronic exposure to Af induces abnormal activation of adhesion signaling pathways, neuritic dystrophy, and synaptic loss (Grace et al., 2002; Grace and Busciglio, 2003). In vivo experiments in transgenic models show the presence of widespread dystrophy in neuronal processes in contact with Af deposits (Tsai et al., 2004; Spires et al., 2005), which contributes to major alterations in neocortical synaptic responses (Stern et al., 2004), yet the apparent lack of correlation between the amount of Af deposition and the severity of dementia strengthened the proposition that soluble, and not fibrillar, forms of A may be responsible for the alterations in neuronal function and viability in AD (Hardy and Selkoe, 2002; Klein, 2002; Tanzi, 2005). This view is supported by experiments showing that soluble A species are present in AD brains and transgenic models (Gong et al., 2003; Kayed et al., 2003; Takahashi et al., 2004; Oddo et al., 2006, Lesné et al., 2006) and that their levels correlate better than plaque density with cognitive impairment (Lue et al., 1999; Naslund et al., 2000). In fact, previous studies indicate that A-soluble species are toxic at low concentrations, reduce synaptic density, induce cognitive dysfunction, and inhibit long-term potentiation (Lambert et al., 1998; Hartley et al., 1999; Dahlgren et al., 2002; Walsh et al., 2002b; Wang et al., 2002).

To perform a side by side comparison of the effect of A species in HCNs, we used homogeneous preparations of AOs, ADDLs, and Af that have been well characterized by EM, HPLC, and immunoreactivity to conformation-dependent antibodies (Lacor et al., 2004; Demuro et al., 2005). We found a very specific synaptic localization of AOs and ADDLs in HCNs. The targeting of AOs and ADDLs to synaptic contacts was fast and accounted for 45–50% of AO total deposits present on HCN cultures after 1 h of incubation. Similar results were obtained with ADDLs, which also show remarkable colocalization with synaptic sites in rat hippocampal neurons (Lacor et al., 2004).

The mechanism by which AOs and ADDLs are targeted to synaptic sites may be a crucial step in the pathological cascade. One possibility is that the high concentration of metal ions at synapses, particularly Cu⁺² and Zn⁺² (Frederickson and Bush, 2001; Mocchegiani et al., 2005; Mathie et al., 2006), "attracts" A oligomers, given the high binding affinity of A for Cu⁺² and Zn⁺² (Bush et al., 1994; Atwood et al., 2000). Then metal–A complexes in the synaptic area may initiate a toxic cascade (Cherny et al., 2001; Frederickson and Bush, 2001), consistent with the synaptic alterations linked to soluble forms of A (Hartley et al., 1999; Walsh et al., 22217). Recent results suggest that ADDLs bind to and reduce the number of NMDA receptors, providing an alternative pathway by which soluble forms of A may cause synaptic failure (Lacor et al., 2005). Notably, most AOs and ADDLs not associated with synapses were found in close contact with cellular membranes, suggesting that soluble A may initiate toxicity not only at synapses but also at multiple cellular locations.

The fast and highly toxic effect of AOs was correlated with a sequence of cellular alterations, which is consistent with the activation of a mitochondrial death pathway, including early changes in MMP and ATP production, gradual decrease in mitochondrial oxidoreductase activity, cytoplasmic translocation of cyt c and AIF, caspase activation, and nuclear condensation (Walker et al., 1988; Cai et al., 1998; Joza et al., 2001; van Loo et al., 2002). These toxic changes were concentration-dependent because lower AO concentrations induced chronic mitochondrial alterations, but not cell death (supplemental Fig. 2, available at www.jneurosci.org as supplemental material). In this regard, chronic and subtle impairment of mitochondrial function by low concentrations of A-soluble species may underlie defective synaptic activity and cognitive impairment in AD patients. Furthermore, transport and localization of mitochondria into neuronal processes, an energy-dependent event, is necessary for the development and maintenance of both spines and synaptic plasticity (Li et al., 2004).

Despite inducing similar changes, the time course of ADDL toxicity was longer. ADDLs required approximately five times longer than AOs to cause similar effects. Structural differences between AOs and ADDLs influencing pore-forming or receptor-binding activities are likely to account for this disparity. An alternative possibility is that the toxic effect of ADDLs could be receptor-mediated, leading to mitochondrial changes by downstream signals over a longer time course.

We found that lowering extracellular calcium delayed significantly the AO toxic process. However, after 24 h AO toxicity in low calcium approached that of AOs in normal calcium. One interpretation is that the rapid toxic response induced by AOs is accelerated by calcium influx (Mattson, 1992; Mattson and Rydel, 1992; Li et al., 1996; Berridge et al., 1998; LaFerla, 2002; Pierrot et al., 2004), but in the absence of calcium the pore-forming properties of A-soluble species (Kagan et al., 2002; Lashuel et al., 22217; Arispe, 2004; Kayed et al., 2004; Quist et al., 2005; Thundimadathil et al., 2005) still trigger the apoptotic process. In this scenario, regardless of calcium influx the progressive formation of A pores in the plasma membrane and internal endomembrane system leads to a general destabilization of ion homeostasis and activation of the apoptotic process.

Supplemental Figure 3A (available at www.jneurosci.org as supplemental material) summarizes the time line of degenerative changes induced by AOs, ADDLs, and Af. AOs and ADDLs at micromolar concentrations result in similar morphological and biochemical changes. AOs exert a faster effect, killing most neurons by 24 h. Five to seven days of incubation are required to generate a similar extent of cell death with ADDLs. Chronic incubation for 10 d and higher concentrations of Af are required to produce generalized dystrophic changes but only modest cell death, whereas nanomolar concentrations of AOs and ADDLs result in chronic mitochondrial dysfunction and minor changes in cell viability.

Supplemental Figure 3B (available at www.jneurosci.org as supplemental material) illustrates a model of the toxic pathway(s) triggered by A-soluble species. AOs and ADDLs are recruited to synapses, possibly by metal ions enriched at synaptic sites and/or synaptic receptors. Another possibility is that A is released at synapses, where it may undergo oligomerization (Gylys et al., 2004). Regardless, the pore-forming activity of A-soluble species could channel a rapid influx of calcium inside cells at synaptic sites and other cellular locations. Mitochondria act as a major buffering system for calcium, but extreme calcium loads lead to the opening of the MTP (Korge et al., 2002; Scorrano et al., 2003; Miyamoto et al., 2005), causing the collapse of the MMP and the release of cyt c and AIF from the mitochondrial matrix to the cytosol where caspases are activated for the execution phase of the apoptotic process. The end stage is illustrated by the complete loss of cell membrane integrity and the release of LDH.

In conclusion, the emerging view of multiple A species capable of deleterious effects at multiple levels coexisting in AD will require a refined therapeutic strategy to address A-mediated neurotoxicity. Additional studies in AD brains will be necessary to assess the synaptic localization of A-soluble species, to establish how the load of A-soluble species changes during disease progression, to determine whether there is a precursor–product relationship among oligomeric and/or fibrillar species, and to understand how each of these factors contributes to neurodegeneration.

	Footnotes

 
Received March 19, 2006; revised April 20, 2006; accepted April 25, 2006.

This work was supported by grants from the Alzheimer's Association (J.B.), the National Institutes of Health (NS21230 to C.G.), and The Larry L. Hillblom Foundation (C.G.). We express our gratitude to Dr. Pascale N. Lacor (Northwestern University, Evanston, IL) for synthetic peptides and Drs. Mary P. Lambert (Northwestern University), William L. Klein (Northwestern University), Ian Parker (University of California, Irvine), and Angelo Demuro (University of California, Irvine) for helpful advice.

Correspondence should be addressed to Jorge Busciglio, Department of Neurobiology and Behavior, University of California, Irvine, 2205 McGaugh Hall, Irvine, CA 92697-4550. Email: jbuscigl{at}uci.edu

DOI:10.1523/JNEUROSCI.1189-06.2006

Copyright © 2006 Society for Neuroscience 0270-6474/06/266011-08$15.00/0

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