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Membrane roughness as a sensitive parameter reflecting the status of neuronal cells in response to chemical and nanoparticle treatments
© Lee et al. 2016
Received: 29 October 2015
Accepted: 20 January 2016
Published: 29 January 2016
Cell membranes exhibit abundant types of responses to external stimulations. Intuitively, membrane topography should be sensitive to changes of physical or chemical factors in the microenvironment. We employed the non-interferometric wide-field optical profilometry (NIWOP) technique to quantify the membrane roughness of living neuroblastoma cells under various treatments that could change the mechanical properties of the cells.
The membrane roughness was reduced as the neuroblastoma cell was treated with paclitaxel, which increases cellular stiffness by translocating microtubules toward the cell membranes. The treatment of positively charged gold nanoparticles (AuNPs) showed a similar effect. In contrast, the negatively charged AuNPs did not cause significant changes of the membrane roughness. We also checked the membrane roughness of fixed cells by using scanning electron microscopy (SEM) and confirmed that the membrane roughness could be regarded as a parameter reflecting cellular mechanical properties. Finally, we monitored the temporal variations of the membrane roughness under the treatment with a hypertonic solution (75 mM sucrose in the culture medium). The membrane roughness was increased within 1 h but returned to the original level after 2 h.
The results in the present study suggest that the optical measurement on membrane roughness can be regarded as a label-free method to monitor the changes in cell mechanical properties or binding properties of nanoparticles on cell surface. Because the cells were left untouched during the measurement, further tests about cell viability or drug efficacy can be done on the same specimen. Membrane roughness could thus provide a quick screening for new chemical or physical treatments on neuronal cells.
Membranes of living cells exhibit many topographic features, such as ruffles, ripples, wave-like pattern propagations, and local stiffness variations. These topographic features depend heavily on the membrane properties as well as the configurations of cytoskeletons. In particular, the membrane biophysics plays essential roles in neuron physiology and pathology. For example, the fluidity of plasma membranes affects the processing of amyloid precursor proteins in neuron cells . Lulevich et al. revealed that amyloid-β (Aβ), the key pathogenic protein of Alzheimer’s disease, increases the stiffness of mouse neuroblastoma cell N2a by using atomic force microscopy . Pan et al. found that Aβ could reduce the membrane roughness of neuroblastoma, and electrical stimulations reversed this effect . But the detailed mechanisms were not clear. Spedden et al. reported that the stabilization of microtubules increased the stiffness of membranes when neurons were treated with paclitaxel (Taxol) . These previous studies showed that the mechanical properties of neuronal cell membranes are sensitive to external physical or chemical treatments.
Gold nanopartices (AuNPs) have been widely used in biomedical applications. Liao et al. demonstrated that negatively charged AuNPs decreased the cytotoxicity of Aβ on human neuroblastoma cells . Ma et al. found that AuNPs of a 16 nm average diameter accelerated the aggregation of Aβ into short fibril bundles. Therefore AuNPs could have the potential to reduce the self-aggregation of Aβ fibrils . Although the blood–brain barrier is considered as a great challenge in nanoparticle-based treatments, nanomaterials still possess high potential for reducing the toxicity of Aβ and other neural toxic peptides related to neurodegenerative diseases . Therefore a simple method to detect the responses of neuronal cells to nanoparticle treatment is also very desirable.
In the present study, we measured membrane roughness of mouse neuroblastoma cell N2a under the treatment of Taxol. In this way we demonstrated that the decrease in the roughness represents the increase of membrane stiffness caused by microtubule translocation. Then we studied the effects of differently charged AuNPs on the membrane roughness of the N2a cells. Finally we conducted a time-lapse measurement of the temporal variation of membrane roughness induced by a hypertonic solution that reduced the membrane tension.
In recent years, membrane roughness has been noticed as a sensitive cellular feature related to various stimulations, including cytoskeletal alteration , blood toxicants , anti-cancer chemicals or nanoparticles [14, 15], proteins related to neurodegenerative diseases , etc. In these works, the membrane roughness was obtained from AFM measurements, and therefore the results could be relevant to the membrane stiffness as well as the cytoskeletal organizations. Because the scanning force of the AFM tip is on the order of nanonewtons, and the image acquisition time is several minutes for one cell, the membrane roughness obtained with AFM could be regarded as a quasi-static mechanical property of the membrane–cytoskeleton complex in a cell.
In the present work we employed NIWOP, an optical profilometry using an ordinary objective as the probe, to obtain cell membrane roughness. Therefore, the measured membrane topography could be considered as a cellular feature under least mechanical perturbations. This is very different from the membrane topography obtained by AFM. Because a NIWOP frame was taken within 5 s, the measured membrane topography could represent the degrees of membrane undulations. Although the membrane roughness variations induced by the alteration of cytoskeletons, such as the microtubule translocation caused by the treatment of Taxol, was measurable, the optical measurement could be more sensitive to the membrane-associated stimulations (e.g., aggregation of Aβ on cell membranes), as we demonstrated in Ref. . Recently it was reported that the aggregation of Aβ precursor protein on cell membranes could be important for the production of Aβ peptides . If such activities of Aβ precursor protein on cell membranes also influence membrane mechanical properties, the measurement on membrane roughness could be used as a label-free assay on this issue. In addition, Aβ and ganglioside GM1 interactions resulting in formation of seeding templates on the membrane rafts may also affect cellular membrane roughness .
The membrane roughness is also sensitive to the adsorbability of nanoparticles on cell membranes. Considering the potential applications of various nanomaterials in the therapeutics of neuronal diseases , a simple and fast assay about the cellular responses to these nanoparticles could be very useful. In addition, because the NIWOP is a bright-field imaging technique, we might also include fluorescent markers or Raman spectroscopy to further exploring the cellular status under the treatment of nanomaterials in a single optical microscope.
Many cellular responses to external stimulations are transient. The time-lapse measurement on membrane roughness could be used to estimate the cellular adaptation rate to environmental variations. In the present work we changed the osmotic pressure of the culture medium by using 75 mM sucrose. Although this treatment reduced the membrane tension and increased the membrane roughness by nearly 1.5-folds, the membrane roughness returned to its original magnitude after 2 h. How the N2a cell adapts itself to compensate the change in the osmotic pressure is an intriguing question to investigate.
Optical profiling techniques with nanometre height accuracy are suitable for living cell characterizations. In addition to the NIWOP technique, membrane roughness might also be acquired by high-speed interferometric imaging techniques, such as live cell interferometry  or phase-shifted laser-feedback interference microscopy . To decipher the variations of membrane roughness in response to stimulations in the microenvironment should also be useful in studying other cell activities, such as stem cell differentiation under the influences of substrate nanofeatures .
In the present work we demonstrated that optical measurement on membrane roughness of neuronal cells could be a sensitive and fast diagnostic technique to reveal the cellular responses to external stimulations. Considering that the membrane physical properties of a neuronal cell play essential roles in neuron degenerative diseases, the membrane roughness can be employed as a quick test of cellular responses to potential drugs and nanomaterial treatments. Because the NIWOP technique is based on bright-field imaging, other optical contrast mechanisms such fluorescence or Raman scattering can be included into this assay for revealing relevant molecular mechanisms.
Setup of the non-interferometric wide-field optical profilometry (NIWOP)
The NIWOP technique  combines the concepts of differential confocal microscopy and wide-field optically sectioning microscopy. We employed the structured-illumination method to produce optical sectioning using a wide-field microscope . The dorsal surface of a cell was placed into the linear region of the axial response curve of the sectioning microscopy, where the intensity is linearly proportional to the height of the sample. Because of the low cytoplasm absorption to the visible light, we had to use a calibration procedure to remove the reflection signal from the bottom surface of the cell . After proper calibrations, membrane topography of an adherent cell could be obtained routinely [25, 26]. In the present work, the membrane roughness was defined as the standard deviation of the measured membrane topography within an 8 × 8 μm2 area near a neurite. The details of the most recent setup of our NIWOP system can be found in Ref. . The depth resolution and dynamic range of the NIWOP system were 52 nm and ~3 μm, respectively. The whole system was placed in a temperature-controlled microscope cage, which provided a constant-temperature environment (37 ± 1 °C) for the live-cell experiments.
We used the cells of a mouse neuroblastoma cell line N2a as the samples in this work. The N2a cell line was obtained from Bioresource Collection and Research Center (Hsinchu, Taiwan). The cells were cultured in Minimum Essential Medium Alpha (MEM-α) (12,571, Gibco, Life Technologies, NY, USA) with 10 % fetal bovine serum and 1 % antibiotic pen-strep-ampho. For long-term observations, the cells were placed into a 100-mm culture dish and the culture area was sealed by a 0.17-mm-thick coverslip surrounded by double-sided adhesive tapes. The volume of the cell region was about 44.5 × 2.5 × 0.07 mm3. With this culture chamber the cells could be kept alive for more than 8 h in the temperature-controlled microscope cage. Before the treatment experiments of Taxol and AuNPs, the medium was replaced with the serum-free MEM-α.
For the observation of microtubules, the cells were fixed with 3.7 % formaldehyde in phosphate-buffered saline (PBS) for 30 min. Then the cells were permeabilized with 0.1 % Triton X-100 in PBS for 5 min and blocked with 1 % bovine serum albumin in PBS overnight. We used the anti-α tubulin antibody conjugate with Alexa Fluor® 488 (Abcam, Cambridge, UK) to label the microtubules in the fixed N2a cells. The fluorescence images were acquired by a confocal microscope (TCS-SP5, Leica Microsystems, Wetzlar, Germany) with a 63×, 1.4 numerical aperture oil-immersion objective.
Scanning electron microscopy (SEM) imaging
We employed a field-emission scanning electron microscope (Nova NanoSEM 200, FEI Company Corp., Hillsboro, OR, USA) to observe the membrane topography on fixed N2a cells. The cells were fixed with 2.5 % glutaraldehyde for 30 min and then washed twice with PBS. The water inside the fixed cells was replaced with ethanol (99.9 %) by gradually increasing the ethanol concentration. The fixed cells were then dried by using a critical-point dryer (EM CPD300, Leica Microsystems, Wetzlar, Germany). The dried fixed cells were coated with 10 nm Au film for better conductance required by SEM imaging.
Gold nanoparticle (AuNP) preparation
The 30 nm AuNPs were purchased from Nanopartz Inc. (Loveland, CO, USA). The surface of the particles carries citrate anions as the capping agents during fabrication, and therefore these particles bear negative charges. We used them as the bare AuNPs in the present work without further modifications. In order to make positively charged AuNPs, the citrate-capped AuNPs were centrifuged at 5000 rpm for 5 min to remove the excess citrate. Then the AuNPs were re-dispersed with 200 μL de-ionized water and then added into 1 mL of 0.1 wt% poly-allylamine hydrochloride (PAH, molecular weight ~15,000, Sigma-Aldrich Corp., St. Louis, MO, USA) aqueous solution. The mixture was incubated overnight, centrifuged at 5000 rpm for 5 min, and then washed with de-ionized water. This procedure was repeated twice. The PAH-coated AuNPs were re-suspended in water and added into the culture medium for cell treatments.
We used NanoBrook 90Plus Zeta Particle Size Analyzer (Brookhaven Instruments Corp., Holtsville, NY, USA) to measure the zeta potentials and hydrated radii of the AuNPs. In the serum-free medium, the average hydrated radius of the bare AuNPs was 188 nm, while that of the PAH-coated AuNPs was 263 nm.
CWL and LLJ performed experiments and conducted data analyses. CWL conducted SEM imaging. LLJ and HJP constructed the optical setup and prepared the samples. YRC, CCC and CHL proposed the original idea, designed the experiments, and helped data interpretations. CWL and CHL wrote the manuscript. All the authors read and approved the final manuscript.
This work was financially supported by the Ministry of Science and Technology of Taiwan (contract MOST 103-2112-M-001-019-MY3).
The authors declare that they do not have any financial or non-financial competing interests.
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- Yang X, Sun GY, Eckert GP, Lee JCM. Cellular membrane fluidity in amyloid precursor protein processing. Mol Neurobiol. 2014;50(1):119–29.View ArticleGoogle Scholar
- Lulevich V, Zimmer CC, Hong HS, Jin LW, Liu GY. Single-cell mechanics provides a sensitive and quantitative means for probing amyloid-beta peptide and neuronal cell interactions. Proc Natl Acad Sci USA. 2010;107(31):13872–7.View ArticleGoogle Scholar
- Pan H-J, Wang R-L, Xiao J-L, Chang Y-J, Cheng J-Y, Chen Y-R, Lee C-H. Using optical profilometry to characterize cell membrane roughness influenced by amyloid-beta 42 aggregates and electric fields. J Biomed Opt. 2014;19(1):011009.View ArticleGoogle Scholar
- Spedden E, White JD, Naumova EN, Kaplan DL, Staii C. Elasticity maps of living neurons measured by combined fluorescence and atomic force microscopy. Biophys J. 2012;103(9):868–77.View ArticleGoogle Scholar
- Liao Y-H, Chang Y-J, Yoshiike Y, Chang Y-C, Chen Y-R. Negatively charged gold nanoparticles inhibit Alzheimer’s amyloid-β fibrillization, induce fibril dissociation, and mitigate neurotoxicity. Small. 2012;8(23):3631–9.View ArticleGoogle Scholar
- Ma Q, Wei G, Yang X. Influence of Au nanoparticles on the aggregation of amyloid-β-(25–35) peptides. Nanoscale. 2013;5(21):10397–403.View ArticleGoogle Scholar
- Zhang M, Mao X, Yu Y, Wang C-X, Yang Y-L, Wang C. Nanomaterials for reducing amyloid cytotoxicity. Adv Mater. 2013;25(28):3780–801.View ArticleGoogle Scholar
- Dehmelt L, Smart FM, Ozer RS, Halpain S. The role of microtubule-associated protein 2c in the reorganization of microtubules and lamellipodia during neurite initiation. J Neurosci. 2003;23(29):9479–90.Google Scholar
- Houk AR, Jilkine A, Mejean CO, Boltyanskiy R, Dufresne ER, Angenent SB, Altschuler SJ, Wu LF, Weiner OD. Membrane tension maintains cell polarity by confining signals to the leading edge during neutrophil migration. Cell. 2012;148(1–2):175–88.View ArticleGoogle Scholar
- Wang X, Ha T. Defining single molecular forces required to activate integrin and Notch signaling. Science. 2013;340(6135):991–4.View ArticleGoogle Scholar
- Tsujita K, Takenawa T, Itoh T. Feedback regulation between plasma membrane tension and membrane-bending proteins organizes cell polarity during leading edge formation. Nat Cell Biol. 2015;17(6):749–58.View ArticleGoogle Scholar
- Girasole M, Pompeo G, Cricenti A, Congiu-Castellano A, Andreola F, Serafino A, Frazer BH, Boumis G, Amiconi G. Roughness of the plasma membrane as a sensitive morphological parameter to study RBCs: a quantitative AFM investigation. Biochim Biophys Acta. 2007;1768(5):1268–76.View ArticleGoogle Scholar
- Kozlova EK, Chernysh AM, Moroz VV, Kuzovlev AN. Analysis of nanostructure of red blood cells membranes by space Fourier transform of AFM images. Micron. 2013;44(1):218–27.View ArticleGoogle Scholar
- Kim KS, Cho CH, Park EK, Jung M-H, Yoon K-S, Park H-K. AFM-detected apoptotic changes in morphology and biophysical property caused by paclitaxel in Ishikawa and HeLa cells. PLoS One. 2012;7(1):e30066.View ArticleGoogle Scholar
- Al-Majmaie R, Kennedy E, Al-Rubeai M, Rice JH, Zerulla D. AFM-based bivariate morphological discrimination of apoptosis induced by photodynamic therapy using photosensitizer-functionalized gold nanoparticles. RSC Adv. 2015;5(101):82983–91.View ArticleGoogle Scholar
- Fang Y, Iu CYY, Lui CNP, Zou Y, Fung CKM, Li HW, Xi N, Yung KKL, Lai KWC. Investigating dynamic structural and mechanical changes of neuroblastoma cells associated with glutamate-mediated neurodegeneration. Sci Rep. 2014;4:7074.View ArticleGoogle Scholar
- Bauereiss A, Welzel O, Jung J, Grosse-Holz S, Lelental N, Lewczuk P, Wenzel EM, Kornhuber J, Groemer TW. Surface trafficking of APP and BACE in live cells. Traffic. 2015;16(6):655–75.View ArticleGoogle Scholar
- Ikeda K, Yamaguchi T, Fukunaga S, Hoshino M, Matsuzaki K. Mechanism of amyloid beta-protein aggregation mediated by GM1 ganglioside clusters. Biochemistry. 2011;50(29):6433–40.View ArticleGoogle Scholar
- Reed J, Troke JJ, Schmit J, Han S, Teitell MA, Gimzewski JK. Live cell interferometry reveals cellular dynamism during force propagation. ACS Nano. 2008;2(5):841–6.View ArticleGoogle Scholar
- Atilgan E, Ovryn B. Reflectivity and topography of cells grown on glass-coverslips measured with phase-shifted laser feedback interference microscopy. Biomed Opt Express. 2011;2(8):2417–37.View ArticleGoogle Scholar
- Zouani OF, Chanseau C, Brouillaud B, Bareille R, Deliane F, Foulc M-P, Mehdi A, Durrieu M-C. Altered nanofeature size dictates stem cell differentiation. J Cell Sci. 2012;125(5):1217–24.View ArticleGoogle Scholar
- Lee C-H, Mong H-Y, Lin W-C. Noninterferometric wide-field optical profilometry with nanometer depth resolution. Opt Lett. 2002;27(20):1773–5.View ArticleGoogle Scholar
- Neil MAA, Juskaitis R, Wilson T. Method of obtaining optical sectioning by using structured light in a conventional microscope. Opt Lett. 1997;22(24):1905–7.View ArticleGoogle Scholar
- Wang C-C, Lin J-Y, Lee C-H. Membrane ripples of a living cell measured by non-interferometric widefield optical profilometry. Opt Express. 2005;13(26):10665–72.View ArticleGoogle Scholar
- Wang C-C, Lin J-Y, Chen H-C, Lee C-H. Dynamics of cell membranes and the underlying cytoskeletons observed by noninterferometric widefield optical profilometry and fluorescence microscopy. Opt Lett. 2006;31(19):2873–5.View ArticleGoogle Scholar
- Chen C-H, Tsai F-C, Wang C-C, Lee C-H. Three-dimensional characterization of active membrane waves on living cells. Phys Rev Lett. 2009;103(23):238101.View ArticleGoogle Scholar