Aβ₄₂ or Aβ₄₀ peptide (Kaneka Eurogentec S.A., Seraing, Belgium) was dissolved in hexafluoroisopropanol (HFIP, Th. Geyer GmbH & Co. KG, Renningen, Germany) and incubated for 2 h at room temperature. Then, peptides were optionally mixed to ratios of Aβ₄₂:Aβ₄₀ of 3:1 (Aβ_3:1), 1:1 (Aβ_1:1), and 1:3 (Aβ_1:3) and aliquoted in Eppendorf tubes. HFIP was evaporated overnight in a vacuum, and the dry peptide films were stored at −70°C until use.

Dried peptide films (Pure Aβ₄₂, Aβ_3:1, Aβ_1:1, Aβ_1:3 and pure Aβ₄₀) were dissolved in 50 mM sodium hydroxide to a 45.5 μM solution and bath sonicated for 5 min. Next, peptide solutions were diluted to 20 μM in black 96-well plates using 60 mM HCl and supplemented with 20 μM Thioflavin T (ThT, Biomol GmbH, Hamburg, Germany). For the vehicle control, the same procedure was repeated but without peptide. The assay was performed using a TECAN Spark plate reader and a humidity cassette (TECAN Group AG, Männedorf, Switzerland) for 6 h at 37°C with excitation at 448 ± 7 nm and emission at 485 ± 20 nm, measuring every 5 min. For data analysis of each experimental run, the intensity of the vehicle control was subtracted from the intensities recorded for the different peptide ratios.

Peptide aggregation protocols were adapted from the protocol by Stine et al. (2011). Briefly, monomeric Aβ₄₂ was prepared by dissolving dried peptide film in cold 0.02% ammonia for 10 min on ice and adding ice-cold sterile ultrapure water to a final concentration of 100 μM. Oligomers of Aβ₄₂ (OAβ₄₂), Aβ_1:1 (OAβ_1:1), and Aβ_3:1 (OAβ_3:1) were obtained by initially dissolving peptide in 0.02% ammonia, followed by sterile ultrapure water and incubation at 4°C overnight. Fibrils of Aβ₄₂ (FAβ₄₂), oligomers of Aβ₄₀ (OAβ₄₀), and Aβ_1:3 (OAβ_1:3) were obtained by adding sterile 10 mM HCl and incubating at 37°C overnight instead. All peptide solutions and aggregates were freshly prepared for each experiment.

Atomic force microscopy (AFM) was performed on a JPK Nanowizard III (Bruker Corporation, Billerica, United States) using ACTA tips (APPNano, Mountain View, United States) with the following properties: tip-radius < 10 nm, spring constant 37 N/m, frequency 300 kHz, 125 μm length, 30 μm width, 4 μm thickness, and an aluminum cantilever coating. Samples were prepared as follows: cleaned mica sheets were glued to microscopy slides using epoxy glue and dried overnight. Then, they were transferred to a laminar-air-flow bench and washed using 300 μL of 96% ethanol (VWR International GmbH, Darmstadt, Germany), and left to dry inside the bench. Mica was cleaved using tape strips for 2–4× until a smooth surface free from cracks was visible. Next, freshly prepared peptide solutions were diluted using ultrapure water to a concentration of 20 μM (monomers, oligomers) or 5 μM (fibrils). Samples were immediately spotted on the mica and incubated for 10 min. Using 100 μL of filtered (0.22 μm) ultrapure water, excess sample solution was washed off. Afterward, samples were placed in a vacuum and stored for a maximum of 16 h before AFM imaging.

Ten microliters drops of peptide solution were placed on calcium fluoride dishes (Korth Kristalle GmbH, Altenholz, Germany) and dried for 30 min in a fume hood. Raman spectra at 30 randomly chosen positions in the middle of the dried drop were acquired with a confocal Raman microscope alpha300R (WITec GmbH, Ulm, Germany) equipped with a 50x objective (NA 0.8) and a 532 m laser set to a power of 20 mW in front of the objective. Integration time was set to 2–8 s. Background and cosmic rays were removed using the ProjectFour software (WITec GmbH, Ulm, Germany). Preprocessed spectra were then imported to Matlab (The Mathworks Inc., Natick, United States). Using the spectra of Aβ₄₂ monomers, oligomers, and fibrils, a cross-correlation analysis was performed to investigate which Raman peaks are subject to sequential change (Lasch and Noda, 2019). With this knowledge, specific peak ratios (1,240 cm⁻¹/1307 cm⁻¹, 1,671 cm⁻¹/1447 cm⁻¹, 1,671 cm⁻¹/1555 cm⁻¹, 1,671 cm⁻¹/1609 cm⁻¹, and 2,935 cm⁻¹/2850 cm⁻¹) were chosen for peak ratio analysis according to the assignments in Supplementary Table S1.

Human SH-SY5Y neuroblastoma cells (Cell lines services, Eppelheim, Germany) were cultured in DMEM with 10% fetal calf serum (FCS) and used up for up to 8 passages (maximum passage 12). Human CCF-STTG1 astroglia (ATCC, Manassas, United States) were cultured in RPMI with 10% FCS and used up for up to 10 passages (maximum passage 12). Human HMC3 microglia (ATCC, Manassas, USA) were cultured in a-MEM with 10% FCS and used for up to 10 passages (maximum passage 12). The human cerebral microvascular endothelial cell line hCMEC/D3 (Cedarlane Labs, Burlington, United States) was cultured on collagen-coated flasks (10 μg/cm²) in EGM-2 medium (Promocell, Heidelberg, Germany) used for up to 6 passages (maximum passage 34). Cells were passaged by trypsinization every 7 days. hCMEC/D3 endothelial cells were used for assays at 30,000 cells/cm², differentiated SH-SY5Y at 45,000 cell/cm², HMC3 microglia and CCF-STGG1 astroglia at 24,000 cells/cm², if not stated otherwise.

All fluorescence staining followed a standardized procedure: after fixation, cells were washed 3× in PBS + 0.05% Tween 20 (PBS-T) for 5 min and permeabilized with 0.2% Triton-X for 5 min. Samples were washed again 3x in PBS-T for 5 min. For antibody staining, samples were first blocked in 5% goat serum and 5% BSA for 20 min. Then, without washing, primary antibody (1:1000 β-III tubulin mouse-anti-human, Thermo Fisher Scientific, Waltham, United States) in blocking buffer (5% bovine serum albumin +5% goat serum in PBS) was added and incubated under gentle shaking at 4°C overnight. Samples were washed 3× in PBS-T for 5 min, and secondary antibody in PBS (1:400 Alexa Fluor 633 goat-anti-mouse) was added and incubated under gentle shaking for 1 h at room temperature. Subsequently, samples were washed 3x with PBS-T for 5 min. For actin staining, samples were incubated after permeabilization and washing with Alexa Fluor 488 Phalloidin or Alexa Fluor 555 Phalloidin under shaking conditions for 1 h at room temperature. Then, samples were washed 3× in PBS-T for 5 min. After the respective staining (antibody or phalloidin or a combination) and washing, samples were counterstained with DAPI (1:100) in PBS under shaking for 5 min at room temperature. After washing 2× in PBS-T and 1x in ultrapure water for 5 min each, samples were mounted in FluorSave (Merck KGaA, Darmstadt, Germany) and dried overnight. Samples were stored at 4°C. Imaging was performed using an inverted confocal laser scanning microscope equipped with 10× (NA 0.45), 20× (NA 0.8), and 40× oil immersion (NA 1.4) objectives (Zeiss, Oberkochen, Germany).

SH-SY5Y neuroblastoma cell differentiation protocols were adapted from existing literature using retinoic acid and brain-derived neurotrophic factor (BDNF), which generates an excitatory neuronal population with glutamatergic and cholinergic markers (Encinas et al., 2000; Dravid et al., 2021; Shipley et al., 2016; Targett et al., 2024). Briefly, SH-SY5Y cells were seeded in T-75 flasks at 10,000 cells/cm² in DMEM supplemented with 10% FCS and left to adhere overnight. On day 1 post seeding, medium was changed to DMEM supplemented with 2.5% FCS, 2 mM glutamine and 10 μM retinoic acid. On day 4 post seeding, medium was changed to Neurobasal™ medium enriched with 50 ng/mL BDNF, 1x B-27(TM) supplement, and 10 μM retinoic acid. On day 7 post seeding, cells were gently passaged, counted, and seeded for experimental use. To verify differentiation, fluorescence staining of β-III tubulin was performed according to the protocol above (Supplementary Figure S2).

The respective cells were seeded in flat-bottom 96-well plates and incubated overnight. The next day, cells were treated with pure and mixed oligomers at 10, 5, 2.5, 1.25, and 0.6125 μM, medium (control), or PBS. Treatment with 100 ng/mL LPS + 20 ng/mL IFN-y (Immunotools GmbH, Friesoythe, Germany) was included for HMC3 microglia. After 24 h, medium was discarded, and fresh medium supplemented with 1 mg/mL 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT) reagent was added and incubated for 4 h at 37°C. Then, medium was discarded again, 100 μL of DMSO was added per well, and the plate was placed on a lab shaker for 15 min. After ensuring the formazan crystals had dissolved, the absorption was measured at 570 nm in a TECAN Spark plate reader (TECAN Group AG, Männedorf, Switzerland). For data evaluation, viability was normalized to the control.

To further verify the differentiation of SH-SY5Y cells, neurite outgrowth was compared between SH-SY5Y neuroblastoma cells and differentiated SH-SY5Y neurons. Briefly, cells were seeded in a 24-well plate left to settle for 24 h. The next day, phase contrast images were acquired using an inverted Leica DMi8 microscope (LEICA microsystems, Wetzlar, Germany) equipped with a 20x objective. Images were then imported to Fiji, converted to 8-bit images and neurite length was measured using the NeuronJ plugin (Meijering et al., 2004; Schindelin et al., 2012). For the investigation of the toxicity of pure and mixed Aβ oligomers, differentiated cells were seeded in 24-well plates in Neurobasal™ medium enriched with 1x B-27(TM) supplement and treated with 10 μM of the respective peptide solution or medium (control) for 24 h. Neurite length was measured as described above.

Briefly, differentiated SH-SY5Y cells were seeded in a 24-well plate and incubated for 24 h, followed by 24 h treatment with 10 μM OAβ₄₂, OAβ_1:3, or medium. Cells were lyzed via the addition of 350 μL TRIzol™ per well, and total RNA was isolated using the Direct-zol RNA MiniPrep Plus Kit (Zymo Research Europe GmbH, Freiburg, Germany) according to the manufacturer; concentration as well as purity were validated photometrically in a TECAN Spark plate reader using the NanoQuant Plate (TECAN Group AG, Männedorf, Switzerland). First-strand synthesis was performed with the Maxima H Minus cDNA Synthesis Master Mix Kit (Thermo Fisher Scientific, Waltham, MA, United States), implementing 250 ng total RNA and following the protocol provided by the manufacturer. Afterward, complementary desoxyribonucleic acid (cDNA) concentration was measured as mentioned above. Cytochrome c (CYC1) messenger RNA (mRNA) level were analyzed via the StepOnePlus Real-Time PCR System (Applied Biosystem, Waltham, MA, United States) using the SYBR Green PowerTrack Master Mix (Thermo Fisher Scientific, Waltham, MA, United States) and 10 ng cDNA. Resulting Ct values were evaluated according to the 2^−ΔΔCt method employing glyceraldehyde-3-phosphate dehydrogenase (GAPDH) as a housekeeping gene. Data were subsequently normalized to the untreated control (Livak and Schmittgen, 2001). The following primer pairs (5′–3′ orientation) were used for amplification: GAPDH forward: CGGGAAGCTTGTCATCAATGG, GAPDH reverse: GGCAGTGATGGCATGGACTG, CYC1 forward: CGGAGGTGGAGGTTCAAGAC, and CYC1 reverse: TAGAGACCTTCCCGCAGTGA. Primer efficiency was routinely validated before the experiment.

The respective cells were seeded on calcium fluoride dishes (Korth Kristalle GmbH, Altenholz, Germany) and incubated overnight. The next day, cells were treated with peptide solutions at 10 μM or medium (control) and incubated for 24 h. Then, cells were fixed in 4% formaldehyde (in PBS) for 10 min, and subsequently washed 3x in PBS. Using a confocal Raman microscope (WITec GmbH, Ulm, Germany) equipped with a 532 nm laser set to a power of 37 mW and a 63× water dipping objective, Raman scans were acquired with an integration time of 0.2 s and a spatial resolution of 500 nm. Background of scans was subtracted using the ProjectFOUR software (WITec GmbH, Ulm, Germany). Scans were then imported to Matlab (The Mathworks Inc., Natick, United States) to remove cosmic rays, smooth the data (Savitzky–Golay filter, window size 9, order 3), and normalized using the Stand Normal Variate method. Next, data was analyzed using the endmember analysis algorithm N-FINDR (Winter, 1999). Briefly, the number of endmembers in the hyperspectral data set was estimated using the noise-whitened Harsanyi-Farrand-Chang (NWHFC) method. End-member spectra were identified by the N-FINDR algorithm and used to calculate end-member abundance maps. Individual abundance maps were overlayed using Fiji. Spectra were plotted, and peak ratio analysis (refer to detailed peak assignment in Supplementary Table S1) was conducted for cytochrome c and/or lipids. Raman imaging was divided into a pre-study to assess feasibility and a subsequent study which encompassed Raman spectra from 3 to 8 cells in total.

Tunneling nanotube (TNT) measurement was adapted from existing protocols (Chakraborty et al., 2023; Kretschmer et al., 2019). Briefly, HMC3 microglial cells were seeded on high-precision glass coverslips (170 ± 5 μm) and incubated overnight. The next day, cells were treated with 10 μM peptide solution or medium (control) and incubated for 24 h. HMC3 cells were then fixed using a two-step fixation protocol: 15 min with 2% formaldehyde and 0.05% glutaraldehyde (Carl Roth GmbH + Co. KG, Karlsruhe, Germany) in PBS, followed by 15 min in 4% formaldehyde in PBS. Subsequently, phalloidin and DAPI staining were performed according to the protocol above, and glass slips were mounted in FluorSave (Merck KGaA, Darmstadt, Germany). Z-stacks were acquired using an inverted confocal laser scanning microscope (LSM900, Carl Zeiss AG, Oberkochen, Germany) using a 20× objective and 0.5 μm step size. For each n and treatment group, 3 z-stacks were acquired at random locations in the sample. Stack scans were then imported to ICY Bioimage analysis software, and TNTs were counted using the TNT annotation tool. A TNT was only counted if the cellular structure hovered above ground level (assessed via z-stack-based spatial resolution of the acquired fluorescence images), if its length exceeded 5 μm, and if its thickness was below 1 μm (Thayanithy et al., 2017; Matejka and Reindl, 2019).

hCMEC/D3 endothelial cells were seeded at 40,000 cells/cm² on 24-well PET 0.4 μm pore inserts (Brand GmbH + Co KG, Wertheim, Germany) in EGM-2 medium (Promocell, Heidelberg, Germany) without VEGF (vascular endothelial growth factor), supplemented with 50 μg/mL ascorbic acid and 1.4 μM hydrocortisone (Caesar & Loretz GmbH, Hilden, Germany). TEER was measured daily using an the Millicell^® ERS-2 (Merck KGaA, Darmstadt Germany) equipped with an EVOM2 electrode (World precision instruments, Sarasota, United States). Plateau TEER was reached on day 3 post seeding, at which point cells were treated with peptide solutions at 10 μM or medium (control) and incubated for 24 h, followed by a final TEER measurement. This experiment was performed in quadruplicate.

The angiogenesis assay was adapted from existing literature (Thomas et al., 2017; Faulkner et al., 2014). Briefly, hCMEC/D3 endothelial cells were starved in DMEM without FCS overnight. Geltrex™ (Thermo Fisher Scientific, Waltham, United States) was thawed at 4°C on ice overnight. The next day, a flat-bottom 96-well plate and 10 μL pipette tips were pre-cooled at −20°C for 30 min, and 2.5 μL of Geltrex™ was pipetted into each well. The plate was then placed at 37°C for 30 min. Meanwhile, hCMEC/D3 cells were passaged and counted. After incubation of Geltrex™ in the plate, hCMEC/D3 cells were seeded in EGM-2 basal medium (Promocell, Heidelberg, Germany). After 4 h, cells were treated with peptide solutions at 10 μM, medium (control), or vascular endothelial growth factor (VEGF, positive control). After 20 h, cells were fixed in 4% formaldehyde (in PBS) for 10 min. Phalloidin staining, followed by DAPI staining, was performed according to the protocol above. Fluorescence images for quantitative analysis were acquired using an inverted Leica DMi8 microscope (LEICA microsystems, Wetzlar, Germany) equipped with a 5× objective. Angiogenesis was assessed using the REAVER script in Matlab (The Mathworks Inc., Natick, United States) with standard settings except for a gray threshold of 0.05, averaging filter size of 500, minimum connected component area of 100, and vessel thickness threshold of 3 (Corliss et al., 2020).

On day 1, 40,000 CCF-STTG1 astroglia were seeded in RPMI +10% FCS on collagen-coated (0.9 mg/mL collagen, 15 μL) basal sides of 24-well inserts (Falcon^® cell culture inserts, 0.4 μm pore size, Corning Inc., Corning, United States) and left to attach overnight. On day 2, hCMEC/D3 endothelial cells (50,000 cells) were seeded on the apical side of the insert membrane in EGM-2. HMC3 microglia (5,000 cells) and differentiated SH-SY5Y neurons (45,000 cells) were seeded in the basal compartment on collagen-coated coverslips (0.1 mg/mL, 900 μL, Corning Inc., Corning, United States) in a-MEM + 10% FCS. On day 3, the medium was exchanged for a-MEM + 2% FCS. After initial TEER measurement on day 4, the basolateral compartment was supplemented with 10 μm Aβ₄₂, Aβ_1:3, 100 ng/mL LPS + 20 ng/mL IFN-γ or medium/PBS (control), respectively, and cells were cultivated for additional 24 h.

TEER was measured on day 5 after 24 h incubation with the respective treatment. TEER measurement was performed in quadruplicate. The medium of the basal compartment was collected for enzyme-linked-immunosorbent-assay (ELISA). Briefly, 800 μL of medium was collected per well and centrifuged at 14,000 rpm for 15 min at 4°C to remove cell debris. The supernatant was frozen at −70°C and thawed 1 h prior to analysis. ELISAs of IL-6 and IL-8 were performed according to the manufacturer’s instructions (Thermo Fisher Scientific, Waltham, United States). For fluorescence imaging and Raman microscopy, cells were fixed according to the TNT cell fixation protocol above or with 4% formaldehyde (in PBS) for 10 min, respectively. Raman microscopy was performed in duplicate. Antibody and phalloidin staining were conducted according to the protocol above on cells fixed with the TNT fixation protocol.

Results are shown as mean values ± standard deviation indicated by error bars. Each experiment included technical triplicates and was performed in triplicate if not stated otherwise. Statistical analysis was performed for the following experiments using the specified test. ANOVA followed by Dunnett post hoc test: DCDRS peak ratio analysis, viability assay, neurite outgrowth assay, PCR analysis of cytochrome c mRNA levels, tunneling nanotube quantification, angiogenesis assay, IL-6 and IL-8 secretion in the BBB model; student’s paired t-test: TEER measurements on endothelial cell monocultures, TEER measurements in the BBB model; two sample t-test: neurite outgrowth of differentiated neurons. Statistical significance is indicated by *p < 0.05, **p < 0.01, and ***p < 0.001 in the figures. If a statistical test was performed, but no significance is indicated, the test was non-significant.

We first investigated the aggregation kinetics of pure and mixed monomeric Aβ₄₂ and Aβ₄₀ in differing ratios by performing a Thioflavin T (ThT) assay, revealing gradual differences in aggregation curves (Figure 2A). While the Aβ₄₀ profile did not reach a plateau in the examined time interval, Aβ₄₂ attained a steady state at 0.87 ± 0.07 a.u. after 65 min. The mixed amyloid curves were distributed between the profiles of pure Aβ₄₂ and Aβ₄₀, differing in steepness of the sigmoid profile and height of the fluorescence plateau. Specifically, profiles of Aβ₄₂:Aβ₄₀ mixtures with a ratio of 3:1 (Aβ_3:1), equal mixtures of both species (Aβ_1:1) and the combination of both species in a 1:3 ratio (Aβ_1:3) reached their plateau after 110 min at 0.45 ± 0.02 a.u, 155 min at 0.31 ± 0.04 a.u., and after 225 min at 0.22 ± 0.05 a.u, respectively.

Subsequently, we prepared oligomers of pure and mixed Aβ₄₂ and Aβ₄₀, (OAβ₄₂, OAβ_3:1, OAβ_1:1, OAβ_1:3, OAβ₄₀) as well as monomers (MAβ₄₂) and fibrils of Aβ₄₂ (FAβ₄₂). Characterization of these aggregate types using atomic force microscopy (AFM) uncovered circular structures for Aβ monomers and oligomers and elongated structures for fibrils (Figure 2B). By measuring aggregate height in each AFM topography, serial increases in size were observable from MAβ₄₂, to OAβ₄₂ and FAβ₄₂, sized 0.29 ± 0.08 nm, 0.69 ± 0.22 nm, and 1.43 ± 0.10 nm, respectively (Figure 2C). OAβ_3:1, OAβ_1:1, OAβ_1:3, and OAβ₄₀ were sized 0.87 ± 0.22 nm, 1.04 ± 0.06 nm, 1.14 ± 0.11 nm, and 0.92 ± 0.03 nm, respectively.

Raman spectroscopy revealed changes in Raman peaks associated with α-helical (1,307 cm⁻¹) and β-sheeted (1,240 and 1,671 cm⁻¹) secondary structure, amide backbone (1,555 cm⁻¹), phenylalanine and tyrosine sidechains (1,607–1,615 cm⁻¹), as well as aliphatic side chains with -CH₂,-CH₃ deformation at 1,447 cm⁻¹, -CH₂ asymmetric stretching at 2,850 cm⁻¹, -CH₂ symmetric stretching at 2,885 cm⁻¹, and symmetric -CH₃ stretching at 2,935 cm⁻¹ (Figure 2D) (Fonseca et al., 2019; Rygula et al., 2013; Mensch et al., 2017; Movasaghi et al., 2007; Kuhar et al., 2021; Jamieson et al., 2018). Next, we employed cross-correlation analysis of Raman spectra of Aβ₄₂ monomers, oligomers, and fibrils. The synchronous spectrum depicted in Figure 2E represents a heatmap of the cross-correlation of all Raman shifts; the symmetry line stems from self-correlation. Thus, the correlation of one specific peak with all other peaks can be identified by examining the synchronous spectrum horizontally or vertically. Figure 2F shows the correlation spectrum at 1671 cm⁻¹, a β-sheet peak, which is positively correlated with another β-sheet peak and negatively correlated with peaks of α-helices, aliphatic side chains, and amide backbone. Using ratios of inversely correlated peaks or peak ratios with constant denominators (2,935 cm⁻¹), steady trends depending on aggregate type were found for each peak ratio (Figure 2G). However, differentiation of pure and mixed oligomers was impossible with this analysis.

Next, we systematically examined the effect of pure and mixed Aβ oligomers on four cell types – endothelial cells, neurons, astroglia, and microglia – to examine differential effects on cell viability, functionality, and metabolism. Endothelial cells form the essential base of the blood–brain barrier, constituting a tight cell monolayer. Whilst OAβ_3:1, OAβ_1:1, and OAβ₄₀ did not affect cell viability, OAβ₄₂ and OAβ_1:3 significantly decreased viability in a concentration-dependent manner, to 67.30 ± 6.53% and 53.96 ± 2.36% at 10 μM, respectively (Figure 3A). Examination of barrier integrity via transepithelial electrical resistance (TEER) measurements exposed a significant reduction of this parameter in endothelial monolayers treated with OAβ₄₂ (from 27.45 ± 4.93 Ωcm² to 20.33 ± 2.18 Ωcm²) and OAβ_1:3 (from 26.40 ± 2.04 Ωcm² to 19.58 ± 4.18 Ωcm²) (Figure 3B). Consistently, the assessment of angiogenesis, encompassing vessel length, area, diameter, and branch points further manifested the indications of toxic effects predominantly induced by OAβ₄₂ and OAβ_1:3 (Figures 3C,D and Supplementary Figure S1).

In the case of differentiated neurons (Supplementary Figure S2), the viability assay depicts concentration-dependent toxicity of OAβ₄₂ and mixed oligomers (Figure 4A). Specifically, OAβ₄₂, OAβ_3:1, OAβ_1:1, and OAβ_1:3 at a concentration of 10 μM reduced cell viability to 69.70 ± 11.53%, 61.70 ± 9.41%, 64.77 ± 10.88%, and 63.03 ± 2.81%, respectively. OAβ₄₀ exposure only led to a reduction of viability to 79.86 ± 8.88%. Further, results of the neurite outgrowth assay exposed an inhibited growth of these protrusions after incubation with mixed oligomers, approximating the effect of OAβ₄₂ (Figures 4B,C and Supplementary Figure S3). We also evaluated the effect of OAβ₄₂ and the mixed oligomer OAβ_1:3, containing a small proportion of Aβ₄₂, on cytochrome c mRNA levels, revealing a 1.16 ± 0.30-fold and 1.78 ± 0.58-fold increase, respectively (Figure 4D). Further, Raman analysis of neurons treated with Aβ oligomers also revealed a trend toward increasing intensities of cytochrome c at 750, 1,129, and 1,585 cm⁻¹ from OAβ₄₀, over mixed oligomers, to OAβ₄₂ (Supplementary Figure S4; Brazhe et al., 2012).

Concerning astroglia, moderate cytotoxicity was registered for OAβ₄₂, OAβ_3:1, OAβ_1:1, and OAβ_1:3 at a concentration of 10 μM (71.17 ± 7.44%, 71.96 ± 2.64%, 82.47 ± 7.15%, and 77.83 ± 3.68%), with OAβ_1:1 leading to the weakest effect, whereas viability was not affected by exposition to OAβ₄₀ (Figure 4E). Further analysis of lipid droplets via confocal Raman microscopy did not reveal differences in lipid droplet distribution (Supplementary Figure S5), however, slight alterations in the corresponding Raman spectra were observed (Figure 4F). Employing peak ratio analysis, we found a lowered ratio of unsaturated to saturated lipids for cells treated with either mixed oligomers or OAβ₄₂, but no trend in alterations in lipid chain length, as shown in Figure 4G.

Similar trends regarding cell viability were also observed in microglia (Figure 5A). While the viability of microglia after exposure to 10 μM OAβ₄₀ or pro-inflammatory stimuli (LPS + IFN-γ) was not significantly reduced (100.80 ± 2.38% and 92.12 ± 1.72%), OAβ₄₂, OAβ_3:1, and OAβ_1:3 showed significant concentration-dependent toxicity (57.41 ± 3.29%, 52.19 ± 9.50%, and 51.83 ± 1.42%), except for OAβ_1:1 (83.13 ± 2.93%). Concerning TNT formation, 38.54 ± 9.07% of cells of the control were connected by at least one TNT, 7.41 ± 2.87% were linked by two TNTs and 8.17 ± 2.74% were joined by more than three TNTs (Figures 5B,C); similar observations were also made for OAβ₄₀ treated cells. However, OAβ₄₂, OAβ_3:1, and OAβ_1:3 treatment significantly increased the total number of TNT-connected cells (64.44 ± 11.00%, 67.56 ± 6.82%, and 62.66 ± 6.29%), as well as the portion of cells connected by three or more TNTs (22.55 ± 1.37%, 26.97 ± 8.25%, and 25.18 ± 7.69%). Moreover, Raman imaging revealed an increased ratio of unsaturated/saturated bonds in lipid spectra in microglia treated with mixed oligomers or OAβ₄₂ (Figures 5D–F), contrasting results obtained from the analysis of astroglial lipid droplets (Figures 4E,F). Furthermore, Raman spectra of microglial lipids droplets displayed a slightly lower chain length after treatment with OAβ₄₂, mixed oligomers, and LPS + IFN-γ. An elevated cholesterol peak was only detected after LPS + IFN-γ exposure.

Observations of toxic effects in single cells sparked a further investigation of the impact of OAβ₄₂ and OAβ_1:3 on a human-based in vitro model of the BBB, composed of endothelial cells in the apical compartment, astroglia lining the basal side of an insert membrane and neurons and microglia in the basolateral compartment (Figure 1). After treatment with OAβ₄₂, OAβ_1:3 or LPS + IFN-γ, fluorescence staining and ELISA (Figures 6A,B) uncovered striking differences between LPS + IFN-γ and Aβ oligomer-treated models. Precisely, microglial and neuronal morphology of OAβ₄₂- and OAβ_1:3-treated models resembled the control, showing intertwined microglia and neurons, as well as extended neurites. Conversely, neurite length was reduced in models treated with LPS + IFN-γ, with microglia circling neurons. Secretion of pro-inflammatory cytokines IL-6 and IL-8 was also strongly increased in these models, whereas no prominent change was observed for samples treated with OAβ₄₂ and OAβ_1:3. TEER was significantly reduced in models treated with OAβ₄₂, OAβ_1:3, as well as LPS + IFN-γ from 32.13 ± 4.83 Ωcm² to 14.36 ± 2.73 Ωcm², 33.83 ± 2.84 Ωcm² to 15.84 ± 3.41 Ωcm², and 31.47 ± 0.87 Ωcm² to 10.11 ± 4.61 Ωcm², respectively (Figure 6C), indicating barrier disintegration in each case. While Raman images of microglia resembled the data acquired from microglial monoculture (Figures 5D, 6D), we identified distinct lipid species in neurons (Figure 6E), which were not detectable in monoculture (Supplementary Figure S4). Further differences between treatments with OAβ_1:3, OAβ₄₂, and LPS + IFN-γ were revealed using peak ratio analysis. In microglia, OAβ_1:3 application led to a shift of lipid spectra toward unsaturated lipids, which was absent for OAβ₄₂. Instead, OAβ₄₂ induced an increase in lipid chain length, which did not occur to the same extent for OAβ_1:3. LPS + IFN-γ treated models displayed only a slight shift toward unsaturated lipids with a simultaneous decrease in chain length (Figure 6F). Lipid spectra acquired from neurons displayed fewer differences, and a trend toward unsaturated or saturated lipids was not as clear; however, chain length was again longest after OAβ₄₂ treatment (Figure 6G). Furthermore, investigation of neuronal cytochrome c revealed elevated levels of cytochrome c, as well as a decreased lipid peak intensity, both of which were strongest for treatment with OAβ_1:3 (Figure 6H).

As protein accumulation is a central characteristic of Aβ-induced pathology, evaluating aggregation kinetics of differing Aβ₄₂:Aβ₄₀ ratios is crucial to investigate their toxicity as co-aggregation of Aβ₄₂ and Aβ₄₀ leads to the formation of oligomers containing both isoforms (Vadukul et al., 2020). Our results clearly indicate a sequential reduction of the aggregation speed of Aβ₄₂ after the addition of Aβ₄₀, implying an inhibitory effect of the shorter peptide variant on Aβ₄₂ fibrillation (Figure 2A) (Chang and Chen, 2014; Braun et al., 2022). Thus, considering the direct impact of aggregate stability, size, and conformation on Aβ toxicity, the observed decrease of plateau height and aggregation speed may contribute to understanding the toxicity of co-aggregated Aβ₄₂ and Aβ₄₀ (Cizas et al., 2010; Chang and Chen, 2014; Vadukul et al., 2020). While prior studies mostly focused on pure oligomers, the formation of mixed oligomers, and especially the ratio of Aβ₄₂:Aβ₄₀, seems to be a crucial factor in neurodegeneration and overall AD-related pathophysiology (Chang and Chen, 2014; Kuperstein et al., 2010; Kwak et al., 2020). The strikingly different aggregation kinetics motivated us to delve further into the structural characterization and composition of Aβ aggregates using AFM and Raman spectroscopy. Our aggregation protocols for monomers, pure and mixed oligomers, as well as fibrils, yielded sizes matching the described range in literature (Figures 2B,C) (Ungureanu et al., 2016; Cizas et al., 2010; Manassero et al., 2016). Despite being a valuable tool for analyzing Aβ aggregates due to its sensitivity to secondary structure, Raman spectroscopy (Figures 2D–G) is rarely used in the context of neurodegenerative diseases. Existing Raman spectroscopic studies have mostly been confined to the examination of fibrillar Aβ (Flynn and Lee, 2018). Notably, Yu et al. (2018) investigated the Aβ aggregation kinetics using surface-enhanced-Raman-spectroscopy (SERS), a technique designed to amplify the Raman signal. However, using SERS affects the location and intensities of Raman peaks, impeding interpretation and making it unsuitable for assessing aggregate conformation. Hence, we sought to explore the potential of Raman spectroscopy in the analysis of amyloid aggregates using drop-coating deposition Raman spectroscopy (DCDRS), entrapping biomolecules in a hydrated environment while decreasing detection limits (Peters et al., 2016; Ortiz et al., 2006). Through cross-correlation analysis, we revealed changes in the secondary structure of beta-amyloid owing to the typical conversion of unordered regions and α-helices to β-sheets (Mallesh et al., 2023). Interestingly, the analysis also uncovered previously unidentified shifts in the Raman spectra. For instance, the amide II band, typically faint due to low scattering effects, was distinguishable for monomeric Aβ₄₂ and faded during Aβ aggregation, indicating an increased rigidity in the amide backbone (Mensch et al., 2017). The decrease in relative intensity of amino acid side chains, such as phenol rings or acyl chains, further suggested constriction of molecular vibrations during this process. We pinpointed these sequential changes in amyloid structure using peak ratio analysis, demonstrating reproducible trends from monomers to fibrils. Overall, Raman spectroscopy offers a straightforward approach to differentiating aggregate types since DCDRS requires minimal sample preparation as opposed to AFM. However, distinguishing aggregate types depending on Aβ₄₂:Aβ₄₀ ratio proved challenging, and further research is needed to address this question.

To examine the effects of Aβ oligomers depending on the Aβ₄₂:Aβ₄₀ ratio, we treated AD-relevant brain cells with pure and mixed oligomers. Importantly, the peptide concentrations used in this study were much higher than physiological levels of soluble Aβ found in brain tissue of AD patients (Roberts et al., 2017). However, such high concentrations are considered necessary to stimulate immortalized cell lines (McCarthy et al., 2016). As main constituents of the BBB, we initially analyzed the cytotoxic effects of pure and mixed oligomers on endothelial cells: only OAβ₄₂ and OAβ_1:3 significantly decreased viability and displayed dose-dependent toxicity (Figure 3A). These findings were confirmed by our investigation of barrier integrity, which showed significant decreases of TEER only after exposure to OAβ₄₂ and OAβ_1:3. This effect has been described for OAβ₄₂, but not for OAβ_1:3 (Figure 3B) (Parodi-Rullán et al., 2020). Further, reduction of angiogenesis has also been depicted in prior reports and was found in our study after exposure to OAβ₄₂, as reported, and OAβ_1:3 (Figures 3C,D) (Parodi-Rullán et al., 2020; Paris et al., 2004). The fact that vascular amyloid deposits mainly constitute Aβ₄₀, combined with the detrimental effects observed in OAβ_1:3 treated endothelial cells, calls for further studies investigating the role of these oligomers for BBB breakdown (Qi and Ma, 2017).

In case of neuronal cells, our results show a decrease in viability and neurite outgrowth upon exposure to OAβ₄₂, consistent with previous reports (Figures 4A–C) (Zhang et al., 2022; Petratos et al., 2008; Krishtal et al., 2017). Equally detrimental effects were observed for each mixed oligomer, aligning with studies by Kuperstein et al. (2010) and Kwak et al. (2020), the latter showing that the Aβ₄₂:Aβ₄₀ ratio drives tau pathology in neurons. Thus, our results underscore the importance of the Aβ₄₂:Aβ₄₀ ratio for AD-associated pathophysiology. Analysis of cytochrome c mRNA levels indicated enhanced expression of cytochrome c after treatment with OAβ₄₂ and OAβ_1:3, amplifying cell death (Chandra et al., 2002). Additionally, Raman imaging of neurons (Supplementary Figure S4) showed that all oligomers, except OAβ₄₀, increased cytochrome c-related Raman peaks, further indicating cytochrome c accumulation. Therefore, our results implicate mitochondrial dysfunction induced by both OAβ₄₂ and oligomers containing only minor amounts of Aβ₄₂, such as OAβ_1:3. These effects may stem from N-methyl-d-aspartate (NMDA) receptor overactivity caused by activation by Aβ oligomers (Gao et al., 2007; Li et al., 2011).

Due to their essential contribution to neurodegeneration and based on the previously reported severe effect of OAβ₄₂, we investigated the effects of differently mixed Aβ oligomers on astroglia (Abramov et al., 2004; Hou et al., 2011). We were able to show prominent effects of such mixed oligomers on these cells, mirroring the results of the viability assay on neurons (Figure 4D). Raman analysis indicated a shift in the composition of astroglial lipid droplets toward saturated lipids instigated by all oligomers except OAβ₄₀ (Figures 4E,F). This inclination is especially interesting, considering astroglia-promoted neurodegeneration via secretion of saturated fatty acids (Guttenplan et al., 2021). Hence, our findings reinforce the hypothesis that Aβ oligomers only containing minor amounts of Aβ₄₂ may be equally toxic as pure Aβ₄₂ oligomers. Besides astroglia, microglia are also strongly linked to AD due to their substantial contribution to neuroinflammation (de Dios et al., 2023). Additionally, especially activated APOE (apolipoprotein E) positive microglia play an important role in Aβ plaque formation and compaction (Kaji et al., 2024; Spangenberg et al., 2019). Our investigation not only confirmed the already reported toxicity of OAβ₄₂ but also uncovered the severe cytotoxic effects of OAβ_3:1 and OAβ_1:3 (Figure 5A) (Pan et al., 2011). The observed proliferative effect (viability above >100% compared to control) after OAβ₄₀ treatment may be linked to a physiological response of the microglia to clear Aβ, albeit this effect was not significant (Fruhwürth et al., 2024). Interestingly, Aβ oligomers also induce the formation of TNTs, serving as a transportation system for Aβ in the central nervous system (Zhang et al., 2021). Previous studies have reported increased TNT-based connections between microglial cells when exposed to Aβ or other toxic peptides like α-synuclein (Chakraborty et al., 2023; Dilna et al., 2021). Our study showed not only an increase in microglia connected with one TNT across the treatment with all oligomers – except OAβ₄₀ – but also a substantial number of cells linked by multiple TNTs (Figures 5B,C). In fact, a previous study found that Aβ₄₂ oligomers are incorporated into endo-lysosomal vesicles, which subsequently transport Aβ between neurons via TNTs (Dilna et al., 2021). Furthermore, other pathological proteins such as prions are also transported inside endo-lysosomal vesicles through TNTs between cells (Zhu et al., 2015). Therefore, it is likely that the TNTs observed in this study served a similar purpose. In addition to TNT formation, microglial lipid metabolism is associated with AD, and we detected an increase in unsaturated lipids in microglial lipid droplets, contrasting the results obtained with astroglia (Figures 5D–F). Interestingly, the lipid profile of LPS + IFN-γ-stimulated microglia markedly differed from cells exposed to oligomeric Aβ, implying different inflammatory cellular responses. These observations are also supported by the viability assay, which showed no significant decrease upon LPS + IFN-γ treatment. Conversely, Aβ oligomers induced a different pathological state, which is highlighted by Raman analysis of lipid droplets. Relative lipid chain length was decreased for cells treated with mixed oligomers, OAβ₄₂, as well as LPS + IFN-γ, however, a strong rise in unsaturated lipids was only observed for mixed oligomers and OAβ₄₂. These alterations in lipid droplet composition toward unsaturated lipids have been identified as a hallmark of inflammation, suggesting production of pro-inflammatory lipids such as arachnoid acid and prostaglandins (Czamara et al., 2017; Chausse et al., 2021). Moreover, the increase of unsaturation is possibly also linked to APOE, which induces abnormal accumulation of unsaturated fatty acids in lipid droplets in AD (Sienski et al., 2021). APOE also facilitates the uptake and compaction of Aβ in the microglial endo-lysosomal system, which leads to the formation of indigestible Aβ aggregates which are released to the surrounding and contribute to plaque growth (Kaji et al., 2024). Thus, APOE not only influences abnormal lipid metabolism but also drives amyloidosis, and future studies should further address the link between the two effects. Meanwhile, LPS + IFN-γ-stimulated cells displayed only a moderate rise in unsaturation and an increase of cholesterol, which was not detected in mixed oligomers and OAβ₄₂-treated cells. Although underlining the differences in the induced inflammatory state, this finding is unexpected as raised levels of cholesterol in microglia are considered a feature of neurodegenerative diseases (Zareba and Peri, 2021; Muñoz Herrera and Zivkovic, 2022). Presumably, the relative increase in cholesterol in Aβ oligomer-treated cells was below the detection limit, while exposure to a strong pro-inflammatory stimulus like LPS + IFN-γ caused a higher relative cholesterol increase. Importantly, the results presented here only encompass the treatment of cultured cells with soluble Aβ oligomers, but not an analysis of intracellular formation or trafficking of these oligomers. Presumably, amyloid precursor protein (APP) is consecutively cleaved by β-secretase and γ-secretase at the lysosomal membrane, leading to the accumulation of Aβ inside lysosomes and subsequent secretion into the extracellular compartment (Tan and Gleeson, 2019). Furthermore, the lysosomal acidic pH promotes aggregation of Aβ and formation of Aβ oligomers already before secretion, causing severe intracellular damage (Schützmann et al., 2021). The role of APOE and lipoprotein flux is particularly interesting in this context, as endocytosis of lipoproteins into lysosomes has been shown to serve as seeding platform for Aβ and to promote plaque growth (Kaji et al., 2024). Therefore, future research investigating Aβ₄₂:Aβ₄₀-ratio-dependent intracellular formation of oligomers, their trafficking and effects may complement the findings presented in this study.

Overall, these monoculture-based studies on endothelial cells, neurons, astroglia, and microglia illustrate the individual effects of mixed Aβ oligomers in the different brain cell types. In each experiment, OAβ_1:3 exposition was equally detrimental to cell viability and function as OAβ₄₂ oligomers, and – in the case of endothelial cells – OAβ_1:3 was the only mixed oligomer type showing similar toxicity as OAβ₄₂. Due to their inherent structural differences, these two oligomer types possibly possess different effects on cells and were, therefore, selected as candidates for a comprehensive evaluation. By extending our study to an in vitro model of the BBB, encompassing all investigated cell types, we further explored differences between OAβ₄₂ and OAβ_1:3 toxicity. We observed a significant drop in TEER after 24 h of exposure to OAβ₄₂, OAβ_1:3, and LPS + IFN-γ, pointing to barrier dysfunction in each case (Figure 6C). Additionally, the absolute decrease of TEER induced by OAβ₄₂ and OAβ_1:3 was more severe than in endothelial cell monocultures. Our observations also align with reported damaging effects of inflammatory stimuli on brain endothelial barrier integrity (Hu et al., 2019). These detrimental effects may lead to both direct damage and the induction of inflammatory responses, which have been reported to shift the phenotype of resting microglia into an activated state (Caldeira et al., 2017). Specifically, literature suggests an amoeboid microglial morphology upon activation, while resting microglia are rather ramified (Wendimu and Hooks, 2022). However, the activation of microglial cells is a highly complex process dependent on various parameters (Gao et al., 2023). In our study, analysis of microglial morphology in the BBB model’s basal compartment revealed differences between oligomer treatment and LPS + IFN-γ stimulation, further suggesting distinctly different immunomodulatory mechanisms (Figure 6A). Accordingly, IL-6 and IL-8 secretion was strongly increased for LPS + IFN-γ treated models but rose only slightly after oligomer exposition (Figure 6B). While these results support both the concept of complex microglial phenotypes and the hypothesis of a dysfunctional microglial phenotype upon stimulation with Aβ, they contrast with evidence specifying an increase of pro-inflammatory interleukin secretion (Franciosi et al., 2005; Kiraly et al., 2023). To gain further insight into changes in cell metabolism, we performed Raman imaging on neurons and microglia (Figures 6D–H). Regarding microglia, the notable rise in the relative amount of unsaturated lipids within lipid droplets triggered by OAβ_1:3 may be linked to involvement in eicosanoid metabolism (Farmer et al., 2020; Khatchadourian et al., 2012). This circumstance is especially interesting, considering free arachidonic acid levels and prostaglandin E2 levels are elevated in AD (Yin, 2023). Conversely, OAβ₄₂ treatment primarily induced an increase of chain length, implying a higher abundance of long-chained lipids in lipid droplets. Notably, apart from polyunsaturated lipids such as prostaglandins, such long-chained saturated lipids are also involved in pro-inflammatory processes mediated by glial cells (Gupta et al., 2012). Moreover, LPS + IFN-γ did not strongly alter the ratio of unsaturated to saturated lipids but decreased relative chain length, further suggesting a different pro-inflammatory mechanism as opposed to oligomeric Aβ. Our findings also reveal the presence of lipids in neurons, which was not observed in monoculture, thereby supporting evidence of lipid transfer between cells in co-culture (Ralhan et al., 2021). Qualitative differences were not as pronounced as in microglia, yet again, OAβ₄₂ led to accumulation of lipids with higher relative chain length, whereas OAβ_1:3 induced enrichment of unsaturated lipids. Interestingly, both phenomena may be evoked by a stress reaction of neurons. Since polyunsaturated lipids are especially vulnerable to peroxidation caused by reactive oxygen species, neurons sequester them into lipid droplets (Bailey et al., 2015). Contrarily, saturated long-chain fatty acids are reportedly highly toxic, alleviated by deposition in lipid droplets, underscoring the complex function of lipid droplets in neurons (Ackerman et al., 2018). Our findings using Raman microscopy also include slight increases in reduced cytochrome c intensities and a reduction of the lipid peak intensity in neurons, particularly associated with OAβ_1:3. These results indicate defects in the respiratory chain and lipid peroxidation, respectively, the latter of which suit the notion of unsaturated lipid rescue into lipid droplets (Abramczyk et al., 2022; Russo et al., 2019).

A possible explanation for the differential biochemical composition of BBB-associated microglia after OAβ₄₂ and OAβ_1:3 treatment as well as the pronounced toxicity of OAβ₄₂ and OAβ_1:3 on endothelial cells and microglia monocultures may be found in the results of the ThT aggregation assay: it demonstrated that Aβ₄₂ is more prone to in situ fibrillation, while Aβ_1:3 forms smaller stable aggregates. Thus, this points toward a dual toxicity of the different oligomeric ratios of Aβ₄₂:Aβ₄₀ – in situ fibrillation of mainly OAβ₄₂, and stabilization of low-Aβ₄₂-high-Aβ₄₀ oligomers, like OAβ_1:3, by their Aβ₄₀ content (Chang and Chen, 2014; Krishtal et al., 2017). Taken together, stable OAβ_1:3 is not only similarly toxic as OAβ₄₂, but these oligomers also seem to cause toxicity via a different mechanism than OAβ₄₂. Furthermore, we observed a less pronounced toxicity of OAβ₄₂ and OAβ_1:3 in neurons and astroglia, which in turn suggests that endothelial cells and microglia are especially prone to Aβ₄₂:Aβ₄₀-ratio-dependent toxicity. Therefore, this study proves that the Aβ₄₂:Aβ₄₀ ratio in oligomers strongly influences cell metabolism and functionality, which is especially crucial considering that Aβ oligomers only containing minor amounts of Aβ₄₂ are formed at the very beginning of AD. Hence, the overall evidence presented in our study clearly questions the Aβ₄₂ oligomer-focused research in the field of AD and reveals a toxicity of Aβ oligomers, which has been previously overlooked.