The mechanism of widespread neuronal death occurring in Alzheimer's disease (AD) remains enigmatic even after extensive investigation during the last two decades. Amyloid beta 42 peptide (Aβ1–42) is believed to play a causative role in the development of AD. Here we expressed human Aβ1–42 and amyloid beta 40 (Aβ1–40) in Drosophila neurons. Aβ1–42 but not Aβ1–40 causes an extensive accumulation of autophagic vesicles that become increasingly dysfunctional with age. Aβ1–42-induced impairment of the degradative function, as well as the structural integrity, of post-lysosomal autophagic vesicles triggers a neurodegenerative cascade that can be enhanced by autophagy activation or partially rescued by autophagy inhibition. Compromise and leakage from post-lysosomal vesicles result in cytosolic acidification, additional damage to membranes and organelles, and erosive destruction of cytoplasm leading to eventual neuron death. Neuronal autophagy initially appears to play a pro-survival role that changes in an age-dependent way to a pro-death role in the context of Aβ1–42 expression. Our in vivo observations provide a mechanistic understanding for the differential neurotoxicity of Aβ1–42 and Aβ1–40, and reveal an Aβ1–42-induced death execution pathway mediated by an age-dependent autophagic-lysosomal injury.
Citation: Ling D, Song H-J, Garza D, Neufeld TP, Salvaterra PM (2009) Abeta42-Induced Neurodegeneration via an Age-Dependent Autophagic-Lysosomal Injury in Drosophila. PLoS ONE 4(1): e4201. doi:10.1371/journal.pone.0004201
Editor: Mark R. Cookson, National Institutes of Health, United States of America
Received: August 19, 2008; Accepted: December 2, 2008; Published: January 15, 2009
Copyright: © 2009 Ling et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was supported by grants from the American Health Assistant Foundation and Sidell-Kagan Foundation to P.M.S. and a fellowship from the John Douglas French Alzheimer's Foundation to D.L. (2005–2007). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
The pathological hallmarks of Alzheimer's disease (AD) are amyloid plaques, neurofibrillary tangles and widespread neuronal loss. A century-old puzzle about the causal relationship between amyloid formation and neurodegeneration remains unresolved due to the lack of a definitive pathogenic pathway linking aggregate-prone proteins with neuronal death. Amyloid beta (Aβ) with 40 and 42 amino acids in length (Aβ1–40 and Aβ1–42, respectively), the main components of amyloid plaques, are aggregate-prone peptides generated from proteolytic processing of amyloid precursor protein (APP). Aβ1–42 has been shown to be more neurotoxic than Aβ1–40 and thus more directly linked to development of AD, . The underlying mechanism of Aβ species-specific neurotoxicity, however, is still absent.
Classically, extracellular deposition of Aβ was thought to be important in AD pathogenesis. More recently, evidence has demonstrated that intraneuronal Aβ may play a crucial role in the early progression of the disease, . Intraneuronal protein aggregates are primarily degraded by macroautophagy (usually referred as to “autophagy”), a lysosome-mediated catabolic pathway responsible for turnover of long-lived proteins and organelles–. Although basal autophagy is undetectable in healthy neurons, the pathway is important to maintain neuronal homeostasis, . Autophagy has been shown to be extensively involved in Alzheimer's–, Parkinson's, lysosomal storage diseases, myopathies, cancers, etc., . However, it is largely unknown if autophagy has a protective or deleterious effect on these diseases–. Activation of autophagy in APP transgenic mice by genetic induction of Beclin1 results in reduced Aβ deposition, suggesting that autophagy functions in Aβ clearance. Mouse models expressing mutant presenilin 1 and APP demonstrated that Aβ peptides are preferentially produced or deposited in autophagic compartments, raising the possibility that a physical interaction may occur between Aβ1–42 and autophagic vesicles. Aβ1–42 expression in nematode muscle cells results in an accumulation of autophagic vesicles that associate with animal paralysis, directly linking Aβ1–42 proteotoxicity with autophagy malfunction. It is thus important to further establish if autophagy malfunction is a cause or an effect of AD pathogenesis. Additionally, the phenotype and fate of neurons with dysfunctional autophagy is poorly characterized.
To identify an Aβ1–42-induced pathogenic pathway, we use the Drosophila Gal4-UAS system to express human Aβ1–40 or Aβ1–42 in two different subtypes of neurons in flies. Both transgenes incorporate a rat preproenkephalin secretory signal peptide to direct secretion after expression and this has been confirmed both in vitro and in vivo, . Aβ1–42 expression induces an age-dependent impairment of neuronal autophagy at a post-lysosomal stage leading to extensive neuronal damage and death. Our data provide the first experimental evidence for an autophagy-mediated neurodegeneration that may be responsible for Aβ1–42-specific neurotoxicity.
Differential neurotoxicity of Aβ1–40 and Aβ1–42
Human Aβ1–40 or Aβ1–42 transgene is expressed in subtypes of Drosophila neurons where soluble GFP is also expressed as a cytosolic reporter that is independent of Aβ expression. GFP labels somas and neuropil of targeted neurons; while Aβ1–42 immunostaining is primarily limited to neuronal somas (Fig. S1). When expression is limited to cholinergic neurons, Aβ1–42 results in a 38.1% of decrease in mean lifespan relative to control (log-rank P<0.0001, Fig. 1A) suggesting a significant Aβ1–42 neurotoxicity. In contrast, Aβ1–40 expression does not shorten fly lifespan. Locomotor activity of Aβ1–42 flies shows an accelerated decrease compared with Aβ1–40 or control flies (Fig. 1B). Similar results were obtained for Aβ1–40 or Aβ1–42 expression limited to GABAergic (and glutamate motor) neurons (not shown). Relative expression levels of Aβ transgenes measured by reverse transcription quantitative PCR (RT-qPCR) show that Aβ1–40 expression is significantly higher than Aβ1–42 (Fig. 1C), thus ruling out the possibility that Aβ1–42-specific neurotoxicity is associated with a higher level of the transgene expression. Cytosolic GFP fluorescence in control (not shown) or Aβ1–40 flies (Fig. 1D) shows relatively homogeneous distribution in neurons. In contrast, region and age-matched Aβ1–42 samples exhibit numerous punctate structures with high GFP fluorescence (fluorescent puncta) relative to the surrounding cytosol with lower GFP fluorescence (Fig. 1E). These puncta show a significantly age-dependent increase (Fig. 1F) that has a negative correlation with animal climbing ability.
(A–B) Aβ1–42 but not Aβ1–40 expression decreases fly lifespan (A) and climbing ability (B) (lifespan assay, N = 953, 633 and 965 for three parallel cohorts of control, Aβ1–40 and Aβ1–42 flies respectively; data are the mean±SEM; climbing assay, N = 160 for all three cohorts). Note that survival rates correlate well with climbing ability in control and Aβ1–40 flies. However, 88% of Aβ1–42 flies at 16 days survive with only 5% maintaining active climbing ability. Aβ1–42 flies thus have accelerated neurological deficits that precede animal death. (C) Levels of Aβ transcripts in fly heads are significantly higher for Aβ1–40 relative to Aβ1–42 (data are the mean+SEM, N = 3 for each group, two-tailed P value by student's t test). (D–E) Cytosolic GFP fluorescence exhibits an even distribution in Aβ1–40 flies (16-day-old adult, D) in contrast to an extensive accumulation of punctate structures in an age- and region-matched Aβ1–42 sample (E). GFP fluorescence in the Aβ1–42 sample is decreased in cytosol (arrowheads) but especially bright in puncta (arrows). Some neuronal somas appear abnormally large (stars). Cellular boundaries also appear to be indistinct (arrowheads). Note that cytosolic GFP expression is independent of the expression of Aβ1–40 or Aβ1–42 thus the fluorescent puncta are not likely to be the structure of Aβ1–42 aggregation. (F) An age-dependent increase of fluorescent puncta in Aβ1–42-targeted neurons (data are mean+SEM, two-tailed P values by student's t test, n = 9 for each group). Scale bars = 5 µm.
Aβ1–42-induced fluorescent puncta are large autophagic vesicles
Electron microscopy was used to identify subcellular structures that could account for the puncta in Aβ1–42 flies. Normal neuronal somas in control flies exhibit well-defined nuclei surrounded by limited cytoplasm (Fig. 2A). However, many neuronal somas in Aβ1–42 flies exhibit an increased volume of cytoplasm and numerous large autophagic vesicles (Fig. 2B). The increased cytoplasmic volume is consistent with the large size of many Aβ1–42-targeted neurons as shown in Fig. 1E. To test if autophagic vesicles represent Aβ1–42-induced puncta, we expressed a transgenic fusion protein between autophagy-specific gene 8a (Atg8a) and GFP. Atg8a-GFP moves from an even distribution in cytosol to a punctate distribution in autophagic vesicles following autophagy induction, . Using a cytosolic RFP reporter to distinguish Aβ1–42-induced puncta from the autophagy reporter, we observe formation of numerous RFP puncta in targeted neurons that extensively colocalize with punctate Atg8a-GFP (Fig. 2C), suggesting that Aβ1–42-induced puncta are autophagic vesicles.
(A) Electron micrograph of typical neuronal somas from a control fly shows the nucleus (N, outlined in blue) surrounded by a limited amount of cytoplasm and no evidence of autophagic vesicles. (B) Electron micrograph of neuronal soma from an Aβ1–42 fly exhibits an abnormally large volume of cytoplasm occupied by an extensive accumulation of large autophagic vesicles (arrowheads). The double arrowheads point to autophagic vesicles derived from the fusion of several smaller vesicles. (C) Cytosolic RFP expression shows Aβ1–42-induced puncta (top panel, arrows) colocalized with punctate Atg8a-GFP (middle panel, arrows), suggesting that they are autophagic vesicles. Scale bars = 1 µm (A–B) or 5 µm (C).
Aβ1–42 expression induces an age-dependent decrease in autophagic degradative function
Healthy neurons are thought to have a high efficiency of autophagy degradation; thus autophagic vesicles are usually undetectable due to their rapid turnover, . To test if induction of normal autophagy could result in accumulation of fluorescent puncta in the absence of Aβ1–42 expression, we fed 1 µM rapamycin, an autophagy inducer, to control flies. Continuous rapamycin feeding does not result in puncta formation in neurons examined in up to 16-day-old adults (Fig. 3A), suggesting that induction of normal autophagy per se does not result in puncta accumulation. Therefore, the numerous puncta in Aβ1–42-targeted neurons (Fig. 3D) are abnormal autophagic vesicles with undigested cargo as indexed by GFP. Electron micrographs reveal numerous autophagic vesicles in neurons from 1-day-old Aβ1–42 flies (Fig. 3B); however, no fluorescent puncta are detectible in neurons at this age (Fig. 3C), suggesting that autophagic vesicles in young Aβ1–42 flies (1–5 days) are functionally normal. The age-dependent increase of fluorescent puncta in Aβ1–42-targeted neurons (Fig. 1F) indicates that the degradative function of autophagy is likely to become progressively impaired with aging. Anti-Aβ immunostaining shows colocalization between fluorescent puncta and Aβ1–42 (Fig. 3E), indicating an accumulation of Aβ1–42 along with other undigested cargo. Aβ1–40 expression under the same experimental conditions does not result in an age-dependent accumulation of fluorescent puncta.
(A) Control flies fed with 1 µM rapamycin up to 16 days exhibit no accumulation of fluorescent puncta in neurons, suggesting that induction of normal autophagy in healthy neurons is not sufficient to induce formation of fluorescent puncta. (B–C) Neurons from 1-day-old Aβ1–42 flies exhibit numerous autophagic vesicles (arrows) in electron micrographs (B) but no fluorescent puncta in confocal micrographs (C), suggesting that autophagic vesicles at an early age can efficiently digest GFP. (D) Confocal micrograph of neurons from 16-day-old Aβ1–42 flies exhibit an extensive accumulation of fluorescent puncta (arrows). (E) Fluorescent puncta (left panel, arrows) colocalize with Aβ1–42 immunostaining (middle panel, arrows) suggesting an association between the two. Scale bars = 5 µm (A, C–E) or 1 µm (B).
Autophagic dysfunction is not due to defective vesicle fusion
Newly formed autophagosomes are known to fuse with lysosome-related vesicles such as autophagic vacuoles, endosomes or lysosomes to acquire catabolic enzymes necessary for their degradative function. To test if Aβ1–42-induced puncta are autophagosomes that have failed in vesicle fusion, we stained fly brains with LysoTracker Red, an acidophilic chemical that marks lysosomes or other lysosome-related vesicles, . Many of the puncta are positively stained by LysoTracker Red (Fig. 4A), suggesting that many, but not all, of the accumulated puncta are post-lysosomal autophagic vesicles. Additionally, we co-expressed a cytosolic YFP reporter along with a chimeric protein, lysosome-associated membrane protein 1 (LAMP1) fused to GFP, in Aβ1–42-targeted neurons. There is an extensive colocalization of Aβ1–42-induced YFP puncta with LAMP1-GFP (Fig. 4B), suggesting that many dysfunctional autophagic vesicles have fused with lysosomes. Some enlarged autophagic vesicles apparently derived from fusion of several smaller vesicles in neurons from Aβ1–42 fly brains (double arrowheads in Figs. 2B and S2) further suggest that the vesicle fusion process is not blocked.
(A) Many GFP puncta in Aβ1–42-targeted neurons are stained by acidophilic LysoTracker Red (left panel, white arrows) while some are not (blue arrows). A high magnification view of an affected neuron (square area) shows a nearly complete colocalization of GFP puncta with LysoTracker Red staining (right two panels) suggesting that many GFP puncta are post-lysosomal vesicles. (B) Cytosolic YFP expression shows Aβ1–42-induced puncta (left panel, arrows) that colocalize with punctate LAMP1-GFP (middle panel, arrows), suggesting that they are post-lysosomal vesicles. Scale bars = 5 µm.
Autophagic vesicles are associated with extensive intraneuronal damage
Normal neurons in young control flies exhibit intact plasma and nuclear membrane and do not show evidence of autophagic vesicles in cytoplasm (Fig. 5A). Neurons in the age-matched Aβ1–42 flies, however, frequently exhibit subcellular damage to plasma (Fig. 5B) or nuclear membranes (Fig. 5C) that are close to large autophagic vesicles. Subcellular damage to organelles such as mitochondria (Fig. S3A) or small trafficking vesicles (Fig. S3B) is also observed in neurons with an accumulation of abnormal autophagic vesicles. Some degenerative neurons in Aβ1–42 flies exhibit large electron lucent areas (Fig. 5D). Consistently, confocal micrographs demonstrate that some Aβ1–42-targeted neurons develop large areas completely devoid of GFP fluorescence (Fig. 5E). These areas are large, irregular, absent of well-defined edges (Fig. 5E) and not bounded by any limiting membrane (Fig. 5D), suggesting that they may represent a type of unlimited digestion or erosive destruction of normal cytoplasmic components. Neurons with erosive areas often lack DAPI staining or the DAPI staining appears smeared (Fig. 5F), consistent with a partially or completely destroyed nucleus (Figs. 5D and S4). Neuropil areas also exhibit damage (Fig. S5).
(A) Normal neurons from control fly brains show continuity in plasma and nuclear membrane and are homogeneous in perinuclear spaces; no large autophagic vesicles in cytoplasm are observed. (B–C) Large autophagic vesicles (arrowheads) in neurons from Aβ1–42 fly brains are associated with extensive subcellular damage to plasma (arrow in B) and nuclear membranes (arrows in C). (D) Degenerative neurons in Aβ1–42 flies exhibit electron lucent areas (stars) occupying a large part of the cytosol. These areas are irregular and not bounded by any limiting membrane distinguishing them from membrane-limited autophagy vacuoles (Av), suggesting that the electron lucent areas may represent uncontrolled digestion or erosive destruction of cytoplasmic components. The nucleus (N) of this neuron is also partially destroyed. (E–F) Confocal micrographs of affected neurons also show large cytosolic areas with weak or absent GFP fluorescence (arrows). DAPI staining is absent (star in F). The large irregular erosive areas (arrows in E–F) lack a well-defined edge, suggesting that they are not membrane-limited compartments devoid of GFP but cytoplasmic areas with unlimited digestion or erosive destruction. Scale bars = 1 µm (A–D) or 5 µm (E–F).
Autophagic leakage contributes to the erosive destruction
Local electron lucent areas in cytosol exhibit a radial dispersion surrounding autophagic vesicles (Fig. 6A), raising the possibility that cytoplasmic erosion may be initiated by a leakage of the catabolic contents of post-lysosomal autophagic vesicles, possibly due to a compromise in their membrane integrity. The multilamellar material in the cytosol of neurons from Aβ1–42 flies provides strong evidence supporting this possibility. Multilamellae, derived from lipid accumulation within autophagic vesicles, , are usually well-packed and contained within the vesicles (Figs. 6B and S6). However, the unexpected appearance of multilamellae in cytosol in the vicinity of autophagic vesicles (Figs. 6C and S7) suggests a leakage of autophagic contents from the vesicles. The erosive areas in degenerative neurons are frequently observed with the appearance of either recognizable autophagic vesicles, multilamellae or both (Fig. S4), suggesting an association between autophagic leakage and erosive destruction of cytoplasm. This subcellular morphology has never been observed in neurons from age-matched control or Aβ1–40 flies. Additionally, the diffuse LysoTracker staining occurs at and beyond the erosive areas with decreased or absent GFP fluorescence in Aβ1–42-targeted neurons (Fig. 6D), indicating that cytoplasmic acidification, likely due to leakage of post-lysosomal vesicles, may precede erosive destruction. Discontinuity of plasma membrane also occurs in some affected neurons (red arrows in Figs. 6C and S7) suggesting membrane destabilization likely due to an abnormality in intraneuronal homeostatic condition.
(A) Local electron lucent area in cytosol (arrow) surrounds autophagic vesicles (arrowheads), suggesting an association between them. (B–C) Multilamellar structures, usually well-packed in autophagic vesicles (arrowhead in B), are unexpectedly seen in cytosol (black arrows in C) where they loosely surround autophagic vesicles (arrowheads in C), suggesting a compromise of the vesicle membrane and a leakage of autophagic contents into cytosol. The red arrow in panel C points to an area in plasma with a discontinuous membrane bilayer. (D) Erosive areas with decreased or no GFP fluorescence (left panel, arrows) exhibit diffuse LysoTracker staining in enlarged regions of surrounding cytosol and numerous LysoTracker-positive puncta (middle panel, arrows), confirming that cytoplasmic acidification and erosive destruction may result from a leakage of compromised post-lysosomal autophagic vesicles. The three orthogonal planes demonstrate that the cytosolic LysoTracker staining is contained within this affected neuron. Scale bars = 1 µm (A–C) or 5 µm (D).
Widespread loss of neuronal integrity occurs following autophagy injury
Consistent with the intact plasma membrane shown in Fig. 5A, fluorescent micrographs of neurons from control (Fig. 7A) and Aβ1–40 (Fig. 7B) samples exhibit homogenous GFP distribution and clear cellular boundaries for neuronal somas observed in flies up to 45 days old. Aβ1–40 flies older than middle age begin to exhibit a small number of puncta in a few neurons but there is no obvious age-dependent increase (Fig. 7B). These morphological features suggest that neurons expressing Aβ1–40 can maintain relatively normal neuronal integrity, consistent with the normal lifespan and climbing ability of Aβ1–40 flies (Fig. 1A–B). Neurons expressing Aβ1–42 in 1-day-old adults also shows homogenous GFP distribution and clear cellular boundaries of neuronal somas (Fig. 7C, 1d). However, Aβ1–42-targeted neurons in flies over 6 days old exhibit a progressive accumulation of dysfunctional autophagic vesicles (GFP puncta, quantitated in Fig. 1F) and a decrease in cytosolic GFP fluorescence followed by indistinct somal boundaries (Fig. 7C, 6d–16d). Taken together, these morphological changes and their relative time scale indicate that Aβ1–42 expression induces an age-dependent deterioration in neuronal integrity resulting from an autophagy-derived injury. The age-dependent loss of neuronal integrity in Aβ1–42 flies correlates well with the reduced lifespan and climbing ability (Fig. 1A–B).
(A) Neurons from young control flies (middle age or earlier) without Aβ expression show homogenous GFP distribution and clear cell boundaries of neuronal somas, no apparent puncta formation. (B) Aβ1–40 expression causes no detectible abnormal autophagy in neurons from young flies (16-day adult, left panel). A few neurons in middle age (31 days) begin to exhibit abnormal autophagy (middle panel, arrows). But no age-dependent deterioration is observed up to 45 days (right panel). (C) Neurons expressing Aβ1–42 exhibit a relatively normal morphology in 1-day adults. Aβ1–42-targeted neurons in over 6-day adults exhibit progressive puncta accumulation, decreased cytosolic GFP fluorescence and loss of clear cell boundaries in affected neurons (arrows) due to an age-dependent autophagic injury. Scale bars = 5 µm.
Autophagy activity modulate Aβ1–42 neurotoxicity
To test if autophagy activity affects Aβ1–42 neurotoxicity, we downregulate autophagy in Aβ1–42 flies by using a loss-of-function allele of autophagy-specific gene1 (Atg1Δ3D). Flies heterozygous for Atg1Δ3D (Atg1+/−) exhibit an expected 50% decrease in Atg1 transcript levels (Fig. 8A). Aβ1–42 flies with the Atg1+/− genotype have a 10.9% increase (log-rank P<0.0001) in mean lifespan compared with Atg1+/+ genotype (Fig. 8B). To rule out the possibility that the lifespan change may result from potential variation in genetic background among fly cohorts, lifespan assay for control flies with and without the Atg1Δ3D allele was also performed in parallel with Aβ1–42 flies. In contrast to Aβ1–42 flies, control flies with the Atg1+/− genotype have a 13.6% decrease (log-rank P<0.0001) in mean lifespan compared with Atg1+/+ genotype (Fig. 8B). Lifespan decrease in normal flies due to autophagy inhibition is consistent with previous observations in mice, , confirming the importance of normal autophagy for animal survival. However, the reverse effects of autophagy inhibition on lifespan between control and Aβ1–42 flies suggest that the significant interaction between Aβ1–42 expression and autophagy activity is not due to any potential influence of genetic background. To additionally rule out the possibility that the Atg1+/− genotype may influence Aβ1–42 expression, the relative expression levels of Aβ1–42 transgene were measured by RT-qPCR. Normalized Aβ1–42 transcript levels in Atg1+/− flies are not significantly different from Atg1+/+ flies (Fig. 8C), suggesting that the lifespan extension in Atg1+/− genotype is not due to a change in Aβ1–42 expression. These data suggest that downregulating autophagy has a protective effect on Aβ1–42 neurotoxicity. In addition, Aβ1–42 flies with the Atg1+/− genotype also show a significantly lower accumulation of fluorescent puncta compared to the Atg1+/+ genotype (Fig. 8D) confirming the important contribution of dysfunctional autophagic vesicles to Aβ1–42-induced neurodegeneration.
(A) Drosophila incorporating a heterozygous loss-of-function allele Atg1Δ3D (Atg1+/−) exhibit a significant decrease in expression levels of Atg1 mRNA in fly brains (data are normalized mean+SEM relative to GAPDH, two-tailed P values by Student's t-test, n = 3 for each group). (B) Control flies with Atg1+/− genotype have a shortened mean lifespan compared to Atg1+/+ genotype (−13.6%, log-rank P<0.0001). In contrast, Aβ1–42 flies with Atg1+/− genotype have extended lifespan relative to Atg1+/+ genotype (+10.9%, log-rank P<0.0001) (data are the mean±SEM). (C) Normalized expression levels of Aβ1–42 transcripts exhibit no significant difference in Aβ1–42 fly heads between Atg1+/+ and Atg1+/− genotypes (data are the mean+SEM, N = 3 for each group, two-tailed P value by student's t test). (D) Aβ1–42 flies with Atg1+/− genotype have significantly fewer fluorescent puncta in targeted neurons relative to Atg1+/+ genotype (fly age is 11 days, data are the mean+SEM, two-tailed P value by Student's t-test, n = 9 for each group). (E) Autophagy activation by rapamycin feeding (1 µM) results in a shorter lifespan for Aβ1–42 flies (−26.0%, log-rank P<0.0001), but has no obvious effect on the lifespan of Aβ1–40 flies (−1.5%, log-rank P = 0.076) relative to flies fed with the same amount of DMSO (data are the mean±SEM). N is the sample size of fly cohorts for each experimental condition.
Autophagy activity can also be downregulated specifically in targeted neurons using an autophagy-specific gene 5 (Atg5) RNAi transgene under control of Gal4-UAS system. To confirm the interaction between Aβ1–42 expression and autophagy activity, we expressed Atg5RNAi transgene (UAS- Atg5RNAi) specifically in Aβ1–42-targeted neurons. Neuron-specific Atg5RNAi expression also results in a lifespan decrease for control flies and again a significant lifespan extension for Aβ1–42 flies (Fig. S8A). Atg5RNAi expression also has no significant effect on Aβ1–42 expression as measured by RT-qPCR (Fig. S8B). To test if autophagy activation has differential effects on flies expressing different Aβ transgenes, Aβ1–40 or Aβ1–42 flies were fed with 1 µM rapamycin to increase autophagy activity. Aβ1–40 flies show no obvious rapamycin-dependent changes in lifespan. However, rapamycin treatment of Aβ1–42 flies results in a significantly shortened lifespan (Fig. 8E), suggesting that enhancement of autophagy may also enhance Aβ1–42 neurotoxicity.
Aging is an independent factor affecting the degradative function of neuronal autophagy
Constitutive autophagic vesicles in healthy neurons are rarely detectable. Consistently, we do not observe autophagy vesicles by electron microscopy or fluorescent puncta in neurons from young control flies in the absence of Aβ expression. However, neurons in control flies at middle age or older begin to exhibit puncta (Fig. S9A–B) consistent with autophagic vesicles observed in electron micrographs of brains from old control flies (not shown). Most of the puncta colocalize with LysoTracker Red staining (Fig. S9C) indicating that they also represent inefficient autophagy vesicles.
Autophagy maintains neuronal homeostasis. It has been shown to protect neurons from degeneration in the absence of any additional aggregated protein,  and improves the survival of animals expressing expanded polyglutamine proteins associated with Huntington disease. The protection may depend on autophagy's ability to efficiently degrade protein aggregates. Consistently, abnormal autophagy has not been detected in patients' brains with Huntington disease, . Unfortunately, not all aggregate-prone proteins are amenable to autophagic degradation, raising the possibility that different types of aggregate-prone proteins associated with different neurodegenerative diseases may differentially affect autophagic clearance. Here we show that two AD-associated peptides, Aβ1–40 and Aβ1–42, have differential effects on neuronal autophagy when expressed in Drosophila neurons. Aβ1–42 induces numerous autophagic vesicles in cytosol with an age-dependent defect in their degradative function and a compromise in their structural integrity that associates with accelerated neurological deficits and a shortened lifespan of the animals. The massive accumulation of autophagic vesicles and their large size may result from cargo storage due to impaired degradative function. Aβ1–40 expression, in contrast, does not show any detectible autophagic changes in neurons or neurological defects in animals, suggesting that Aβ1–40 is likely to be processed efficiently by neuronal autophagy. The differential effects of Aβ1–42 and Aβ1–40 on neuronal autophagy could be the underlying cause of their differential neurotoxicity. This finding may explain the paradoxical observations that APP proteolysis primarily generates Aβ1–40 in neurons, while it is predominantly Aβ1–42 that exhibits intraneuronal accumulation, .
Abnormal autophagy is a prominent neuropathological phenotype of AD, . The abnormality has been proposed to result from a failure of fusion between autophagosomes and lysosomes making them unable to complete their degradative function, , , . Here we provide compelling evidence that Aβ1–42-induced dysfunction of autophagic vesicles may occur at a post-lysosomal fusion stage. Moreover, the multilamellar structures outside of autophagic vesicles along with cytosolic acidification indicate a compromise of and then a leakage from the post-lysosomal vesicles. These events cause further membrane and organelle damage as well as erosive destruction. The detailed pathogenic processes for the erosive destruction are currently unknown. However, this abnormal phenotype in our Drosophila model is consistent with previous histopathological observations of AD brains where affected neurons with an intracellular accumulation of Aβ1–42 experience cell lysis that is associated with the appearance of lysosomal enzymes in cytoplasm. Thus the pathological features we observed are not species-specific, but may reflect a common consequence of Aβ1–42 pathology in neurons.
We also observe that normal aging decreases the efficiency of autophagic degradation in agreement with previous reports, . Due to this common cellular consequence, aging could thus facilitates Aβ1–42 neurotoxicity, or vice versa, in agreement with similar neuropathological features shared by normal aging and AD. Autophagy inhibition via a haploinsufficiency of Atg1 or targeted neuron-specific expression of Atg5RNAi extends lifespan of Aβ1–42 flies in contrast to the deleterious effects on flies without Aβ1–42 expression, suggesting that Aβ1–42 expression may shift neuronal autophagy to a pathogenic condition. Taken together, we propose an autophagy-mediated pathogenic process where functional and intact autophagy has an early pro-survival effect that shifts to a later pro-death effect due to chronic deterioration in both degradative function and structural integrity. Our data suggest a mechanism for a dual role of autophagy that has been observed in different cellular contexts, .
In summary, we express human Aβ1–42 and Aβ1–40 separately in Drosophila neurons revealing an Aβ1–42-dependent pathogenic pathway linking autophagy malfunction with progressive neurodegeneration. Aβ1–42 impairs the degradative function and structural integrity of neuronal autophagy but not the maturation process of autophagic vesicle fusion. A death execution pathway may be triggered by leakage of post-lysosomal autophagic vesicles leading to cytosolic acidification, subcellular damage to membranes and organelles, and erosive destruction of cytoplasm. Even though the direct expression of Aβ constructs containing a preproenkephalin secretory signal in Drosophila neurons may not mirror the normal conditions of Aβ generation from full-length of APP, our observations suggest a mechanism for differential neurotoxicity of Aβ1–42 and Aβ1–40 as well as a cellular pathway that is responsible for Aβ1–42-induced neuronal death. Future studies will be required to uncover detailed molecular mechanisms underlying these cellular changes.
Materials and Methods
Drosophila melanogaster was raised at 25°C (embryonic and larval stages) and 28°C (adult stage) using standard methods. Female adults were used for all experiments. Gal4 driver lines were 7.4 kb Cha-Gal4 targeting all cholinergic neurons and 3.2 kb Gad1-Gal4 targeting all of the glutamic acid decarboxylase 1 (Gad1) expressing neurons. UAS responders were UAS-Aβ1–40, UAS-Aβ1–42, UAS-GFPS65T, UAS-eYFP (Bloominton Stock Center), UAS-RFP, UAS-LAMP1-GFP, UAS-Atg8a-GFP, UAS-Atg5RNAi, and Atg1Δ3D.
Groups of 20 individual flies were collected within 24 hours of eclosion and placed in fresh food vials (2.3 cm diameter×8.4 cm height). Vials were incubated at 28°C and live flies were regularly transferred to new food vials while the number of dead flies was counted. Parallel cohorts were assayed at the same time under the same conditions and the experimenter was blinded to the genotypes or experimental conditions. The survival rates were calculated using the LIFETEST procedure and log rank test in SAS software. The relative changes (%) of mean lifespan between parallel cohorts were calculated as [(Mean-MeanRef.)/MeanRef]*100%.
Reactive climbing assay is as described with slight modifications. Ten female flies were placed in a plastic vial and gently tapped to the bottom. The number of flies that reached a mark at the top of the vial within 10 seconds was recorded. Ten trials were performed to get an average number for each time point. The data represent combined results from a cohort of flies tested every 5 days for each genotype.
Adult fly brains were dissected in phosphate buffered saline (PBS), and fixed in PBS with 4% formaldehyde for 30 minutes for microscopic observation of endogenous GFP (or RFP/YFP). For LysoTracker staining, freshly dissected fly brains were incubated in PBS with 100 nM LysoTracker Red (Molecular Probes) for 15 minutes, washed 2 times with PBS and immediately observed. For Aβ immunostaining, dissected brains were fixed in PBS with 4% paraformaldehyde at 4°C overnight. Fixed brains were permeabilized in 1% Triton X-100 in PBS for 5 hours and treated with 70% formic acid in PBS for 20 minutes, and immunostained with anti-Aβ antibody 4G8 (Signet Laboratories) followed by detection with a Texas-Red conjugated secondary antibody. Samples were observed by confocal microscopy (Zeiss LSM 510). For quantitative morphological analyses, objects (fluorescent puncta) were manually counted in representative confocal images using ImageProPlus (Media Cybernetics). At least 3 non-overlapping optical sections were sampled from confocal Z-sections taken from 3 individual specimens. The counter was blinded to sample identities (such as genotypes, ages, or experimental conditions). Data were analyzed by ANOVA followed by pairwise Student's t-tests corrected for multiple comparisons.
Dissected brains were fixed in 1.6% paraformaldehyde with 2% glutaraldehyde and 0.06 M cacodylate buffer at 4°C for 24 hours. Brains were post-fixed in osmium and embedded in eponate. Ultrathin sections were stained with uranyl acetate and Sato's lead. Specimens were observed with an FEI Tecnai transmission electron microscopy. Independent observations from 3–5 animals were performed for each experimental condition.
Rapamycin feeding was as described. Flies were allowed to mate on normal fly food for 2–3 days and then transferred to fresh food containing 1 µM rapamycin (Sigma) or an equal volume of DMSO (vehicle for dissolving rapamycin) for egg collection, embryogenesis and larval growth. Female flies were collected within 24 hours after eclosion and incubated at 28°C in vials containing food supplemented with rapamycin or DMSO for lifespan assays.
Reverse Transcription and quantitative real-time PCR
Fifty fly heads were collected on dry ice and total RNA was isolated using RNA STAT-60 (Tel-Test). RNA samples were treated with DNase I to remove genomic DNA and reverse transcribed to cDNA using the iScript cDNA Synthesis Kit (Bio-Rad). Three biological replicates of the same experimental condition were performed. Gene-specific transcription levels were determined in triplicate by real-time PCR using SYBR Green Supermix (Bio-Rad) and an IQ5 real-time PCR machine (Bio-Rad). Primers were 5′-CTTCCAGGCGTCGCATCC-3′ and 5′-GTCTTCAGTTGTCCCTTCTTCG-3′ for Drosophila Atg1, 5′-CTACGCTATGACAACACCGC-3′ and 5′-AGACTTTGCATCTGGCTGCT-3′ for Aβ1–42/ Aβ1–40 transgenes, or 5′-CCACTGCCGAGGAGGTCAACTAC-3′ and 5′-ATGCTCAGGGTGATTGCGTATGC-3′ for Drosophila glyceraldehyde-3-phosphate dehydrogenase (GAPDH) as a reference. Ct values of real-time PCR were analyzed by a custom SAS program relying on a published algorithm to calculate mean normalized expression relative to GAPDH. Representative data from 3 separate experiments are presented as mean±SEM. Two-tailed P values were calculated by Student's t-test between parallel groups.
Coexpression of cytosolic GFP reporter and Aβ1–42 (or Aβ1–40) in Drosophila brains using UAS-Gal4 technique. An optic lobe of an adult fly brain is shown here. Soluble GFP fluorescence (green) distributes in both neuronal somas and neuropil (outlined in cyan). Only neuronal somas are additionally labeled by Aβ1–42 immunostaining using anti-Aβ antibody 4G8 (red). DAPI staining cellular nuclei (blue) is confined to cell somas. Scale bar = 20 µm.
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Large autophagic vesicles are formed by vesicle fusion. (A–B) The double arrowheads indicate autolysosomes formed from the fusion among autophagosomes and lysosomes in affected neurons from Aβ1–42 flies. The red arrow in B points to a damage of the plasma membrane. (C) A high power view of an autophagic vesicle derived from the fusion of several smaller vesicles. Note that these post-fusion autophagic vesicles (A–C) all have an enclosing outer membrane and a distinct inner membrane around each individual smaller vesicle, suggesting that vesicular fusion is normal. Scale bars = 1 µm (A–B) and 200 nm (C).
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Autophagy-associated subcellular organelle damage. (A) An affected neuron shows many autophagic vesicles (multilamellar bodies, arrowheads) along with numerous mitochondrial fragments (red arrows) suggesting mitochondria damage. (B) An affected neuron exhibiting numerous disrupted membrane structures (red arrows), likely derived from damaged small transport/secretory vesicles. Some normal-looking intact vesicles are still visible (black arrows). The arrowheads indicate different sized autophagic vesicles (multilamellar bodies). Av = autophagy vacuole. Scale bars = 1 µm.
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Cytoplasmic erosive areas in degeneratve neurons associate with autophagic injury. (A and B) Some neurons from Aβ1–42 flies have lost their normal subcellular structures and developed multiple electron lucent areas (stars), suggesting that extensive cytoplasmic erosion associates with neurodegeneration. Some of the erosive areas exhibit recognizable autophagic vesicles (blue arrowheads) or multilamellar materials (red arrowheads) or both suggesting that cytoplasmic erosion associates with autophagic injury. Scale bars = 1 µm.
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Aβ1–42-induced damage in neuropil areas. (A) Typical neuropil area from a control brain. (B) Most neuropil areas from Aβ1–42 fly brains have similar morphology compared to control samples. Mitochondria (stars) are the prominent organelles in neuropil areas. (C) Some electron lucent areas (arrows) are present in Aβ1–42 samples suggesting damage. (D) A large electron lucent area (black arrow) shows more extensive damage in neuropil. The red arrow points to a multilamellar structure possibly resulting from membrane disturbance or leakage of nearby autophagic vesicles. Scale bars = 1 µm.
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Whorl-like multilamellae in an autophagic veiscle. Multilamellae can spontaneously form from lipids accumulating within autophagic-lysosomal vesicles ,  especially at acid pH . There are several different sized multilamellar stacks formed independently in a large autophagy vesicle. Disruption or incomplete digestion of membranes from many small vesicles sequestered within autophagy vesicles is the source of multilamellae (arrows). Scale bar = 0.5 µm. Supporting References: 1. Lajoie P, Guay G, Dennis JW, Nabi IR (2005) The lipid composition of autophagic vacuoles regulates expression of multilamellar bodies. J Cell Sci 118: 1991–2003. 2. Hariri M, Millane G, Guimond MP, Guay G, Dennis JW, et al. (2000) Biogenesis of multilamellar bodies via autophagy. Mol Biol Cell 11: 255–268. 3. Hayakawa T, Makino A, Murate M, Sugimoto I, Hashimoto Y, et al. (2007) pH-dependent formation of membranous cytoplasmic body-like structure of ganglioside G(M1)/bis(monoacylglycero)phosphate mixed membranes. Biophys J 92: L13-16.
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Disturbance of membrane bilayers in affected neurons from Aβ1–42 flies. (A and B) Destabilized plasma membranes form lamellar structures (red arrows), suggesting an abnormality in intraneuronal homeostasis. Nuclear membrane has also been disrupted (black arrows in A). The arrowhead in (A) points to an autophagic vesicle. An irregularly dispersed multilamellar structure in cytosol (black arrow in B) likely results from a damaged autophagy vesicle not visible in this section. In addition, the neuron in (B) has an indistinct nuclear membrane possibly also due to abnormal homeostasis. N is nucleus. Scale bars = 1 µm.
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Autophagy inhibition by Atg5RNAi in targeted neurons has reverse effects on lifespan of control and Aβ1–42 flies. (A) Neuron-specific inhibition of autophagy by expression of an Atg5RNAi transgene in targeted neurons results in a decreased lifespan for control flies (−11.3%, log-rank P = 0.0003) and an extension of lifespan for Aβ1–42 flies (+12.4%, log-rank P<0.0001) (Data presented are the mean±SEM). N is the sample size of fly cohort for each experimental condition. (B) Normalized expression levels of Aβ1–42 transcripts exhibit no significant difference in Aβ1–42 fly heads between with and without Atg5RNAi expression (data are the mean+SEM, N = 3 for each group, two-tailed P value by student's t test).
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Decreased efficiency in autophagic degradation is a consequence of normal aging. (A) Middle-aged (31 days) control flies show occasional GFP puncta (arrow) indicative of abnormal autophagic degradation. (B) Control flies near the end of their lifespan (51 days) exhibit an increased number of GFP puncta (arrows) in brains. (C) Most of the puncta in old control flies (51 days) colocalize with LysoTracker Red staining (white arrows), suggesting that they are inefficient autophagic vesicles. Scale bars = 5 µm.
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We thank our City of Hope colleagues Elvia Gutierrez, John Hardy, Kazuo Ikeda, Marcia Miller and Rodney Williamson for their experimental support and discussion. We also thank Dr. Helmut Krämer (UT Southwestern Medical Center, TX), Dr. Brian Howell (National Institute of Neurological Disorders and Stroke) and the Bloomington Drosophila Stock Center for providing Drosophila lines.
Conceived and designed the experiments: DL PMS. Performed the experiments: DL. Analyzed the data: DL PMS. Contributed reagents/materials/analysis tools: DL HJS DG TN PMS. Wrote the paper: DL PMS. Provided experimental suggestions: HJS DG TN.
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