- Open Access
Impact of nanoparticle surface functionalization on the protein corona and cellular adhesion, uptake and transport
Journal of Nanobiotechnology volume 16, Article number: 70 (2018)
Upon ingestion, nanoparticles can interact with the intestinal epithelial barrier potentially resulting in systemic uptake of nanoparticles. Nanoparticle properties have been described to influence the protein corona formation and subsequent cellular adhesion, uptake and transport. Here, we aimed to study the effects of nanoparticle size and surface chemistry on the protein corona formation and subsequent cellular adhesion, uptake and transport. Caco-2 intestinal cells, were exposed to negatively charged polystyrene nanoparticles (PSNPs) (50 and 200 nm), functionalized with sulfone or carboxyl groups, at nine nominal concentrations (15–250 μg/ml) for 10 up to 120 min. The protein coronas were analysed by LC–MS/MS.
Subtle differences in the protein composition of the two PSNPs with different surface chemistry were noted. High-content imaging analysis demonstrated that sulfone PSNPs were associated with the cells to a significantly higher extent than the other PSNPs. The apparent cellular adhesion and uptake of 200 nm PSNPs was not significantly increased compared to 50 nm PSNPs with the same surface charge and chemistry. Surface chemistry outweighs the impact of size on the observed PSNP cellular associations. Also transport of the sulfone PSNPs through the monolayer of cells was significantly higher than that of carboxyl PSNPs.
The results suggest that the composition of the protein corona and the PSNP surface chemistry influences cellular adhesion, uptake and monolayer transport, which might be predictive of the intestinal transport potency of NPs.
Commercial, therapeutical and technological interests in engineered nanoparticles (NPs) are still increasing because of their unique physicochemical properties that make them promising materials for a wide range of new applications. NPs are currently being used in the agri-food sector in particular within domains like food processing, packaging, and as nutraceutical delivery systems [1,2,3]. The unique size-related properties may also pose a risk to human health because of their interactions with biomolecules, cells and organs, potentially leading to adverse outcomes [4, 5]. The oral route of exposure is considered one of the main exposure routes, especially for NPs exploited in agri-food applications. To assess the likelihood of NPs to internalize and cross the intestinal epithelial barrier several in vitro intestinal epithelial models have been developed [6,7,8,9]. Rapid screening of the intestinal transport potential of NPs is important in a tiered risk assessment or grouping approach .
The cellular uptake/transport of NPs is highly dependent on both the intrinsic and extrinsic properties of NPs. It is well known that intrinsic NP properties, such as size  and surface modifications affect cellular uptake [11, 12]. Upon contact with biological matrices like gastrointestinal juices and body fluids NPs are immediately covered with proteins generating the so-called protein corona . The composition of the protein corona formed on the NPs surfaces is highly influenced by the physicochemical properties of the NPs [14, 15]. Consequently, the NP corona is considered as one of the major players affecting the biological interactions of the NPs, including their cytotoxicity, uptake and transport [14, 16, 17]. Additionally, the correlation between NP properties and their cellular uptake/transport appears to be cell type dependent, indicating that different kinds of uptake/transport mechanisms could be in place [18, 19]. Due to these complexities, no key descriptor has been identified so far for NP uptake/transport.
Here we aimed to study the effects of the size and surface chemistry of NPs on the protein corona formation and their subsequent cellular adhesion, uptake and transport. Several methods are available to study the cellular interactions of NPs at a single-cell level. High content (HC) imaging analysis has proven to be a highly successful and powerful tool in the field of drug discovery and toxicology, but it has rarely been used to study the behaviour and uptake of NPs [20, 21]. Here, HC imaging was used to study the cellular associations of fluorescently labelled, negatively charged, polystyrene nanoparticles (PSNPs) on a single-cell level, using Caco-2 monolayers as an in vitro method that mimics the human intestinal epithelium. Also, the transport of these PSNPs was assessed to gain insights into the correlation between the cellular adhesion/uptake and transport of these PSNPs. Lastly, the composition of the protein corona was quantitatively determined using label-free liquid chromatography mass spectrometry (LC–MS/MS).
Two 50 nm negatively charged, red fluorescently-labelled PSNPs with different surface modifications were obtained from Magsphere® (Pasadena, USA). Namely; 2.5% w/v sulfonated particles and 2.5% carboxylated PSNPs, further referred to as 50 nm (-SM) and (-CM), respectively. 50 nm and 200 nm negatively charged, 2.5% w/v yellow-green fluorescently-labelled carboxylated PSNPs (Fluoresbrite®) were obtained from Polysciences (Warrington, USA), further referred to as 50 nm (-CP) and 200 nm (-CP). All PSNPs suspensions were stored at 4 °C and all experiments were performed using the same batch of PSNPs. Serial dilutions of the PSNPs were freshly prepared for every experiment in complete cell culture medium. Absence of detectable leakage of the fluorophores from the PSNPs used was confirmed by centrifugation of NPs after 24 h incubations in cell culture medium at 37 °C .
Adherent human epithelial colorectal adenocarcinoma cells (Caco-2; ATCC® HTB-37™), were used at passage numbers 25–40. They were cultured and maintained in 75 cm2 cell culture flasks (Corning®; New York, USA) at 37 °C in a humidified 5% CO2 atmosphere (HERAcell 240 incubator; Marietta, USA). Complete cell culture medium was prepared by supplementing Dulbecco’s Modified Eagle Medium (DMEM) culture medium (LONZA; Verviers, Belgium) with 10% (v/v) heat inactivated Foetal Bovine Serum (FBS) (Gibco®, Life technologies; New York, USA), 1% (v/v) of Penicillin–Streptomycin (Sigma-Aldrich; Steinheim, Germany), and 1% (v/v) of MEM Non-Essential Amino Acids (NEAA) (Gibco®, life technologies; New York, USA). The complete medium is further referred to as DMEM+.
Physicochemical characterization of PSNPs
Size and surface charge of PSNPs were characterized using dynamic light scattering (DLS) and zeta-potential measurements, respectively. Briefly, DLS measurements were performed on 10 µg/ml PSNPs suspended in water and/or DMEM+ using an ALV dynamic light scattering setup (ALV-Laser Vertriebsgesellschaft; Germany), consisting of a Thorn RFIB263KF photomultiplier detector, ALV-SP/86 goniometer, ALV 50/100/200/400/600 μm pinhole detection system, ALV7002 external correlator, and a Cobolt Samba-300 DPSS laser. Each sample was measured 10 times for 30 s at an angle of 90°. The results are expressed as the hydrodynamic diameter that was calculated using AfterALV® software (AfterALV 1.0d, Dullware; USA). The zeta-potential was measured using a Malvern Zetasizer 2000 (Malvern Instruments; Malvern, UK) on 10 µg/ml PSNPs suspended in DMEM+. All samples were analysed in triplicate.
In vitro sedimentation, diffusion and dosimetry (ISDD) model for PSNPs
The deposited fraction of the administered doses of the PSNPs (target cell dose) was calculated using the In vitro Sedimentation, Diffusion and Dosimetry (ISDD) model . The following parameters were used as input in the ISDD model: the hydrodynamic diameters of the PSNPs in water and DMEM+ measured by DLS (Table 1), medium column height (10.9 mm), temperature (310°K), media density 1 g/ml and media viscosity 0.0009 N s/m2 [23, 24].
Cytotoxic effects of the PSNPs were determined using a Cell Proliferation Reagent WST-1 (Roche; Mannheim, Germany). Each well was seeded with 1 × 105 cells/cm2 in DMEM+ in 96-well flat bottom plates (Greiner bio-one; the Netherlands). Plates were incubated at 37 °C, 5% CO2 for 24 h. Attached cells were then exposed to 100 µl/well of freshly prepared serial dilutions of 50 nm- (-SM), (-CM), (-CP), and 200 nm (-CP) PSNPs (15, 25, 50, 75, 100, 200, 250, 500 and 750 µg/ml) for 3 and 24 h. Afterwards the exposure medium was discarded and 10 µl of WST-1 solution was added with 90 µl of DMEM+ (without phenol red) to each well. The plates were incubated for 24 h at 37 °C, 5% CO2 and absorbance was read at 490 nm and 630 nm on a plate reader (BioTek Synergy™ HT Multi-Mode Microplate reader; USA). Cell viability for each concentration of PSNPs was expressed as a percentage of the control. DMEM+ was used as a negative control and Triton-X100 (0.25%) (Sigma) was used as a positive control that decreased the viability to 29 ± 0.2%.
PSNP cellular adhesion and uptake studies and HC imaging
A cell suspension of 5 × 104 cells/cm2 was seeded in 96-well flat bottom black plates (Grenier bio-one; Frickenhausen, Germany) and incubated at 37 °C, 5% CO2 for 24 h. Subsequently, the culture medium was aspirated and cells were exposed to 100 µl/well of 15, 25, 50, 75, 100, 200 and 250 µg/ml of each of the PSNPs (n = 2) for 10, 20, 30, 60, and 120 min for the (-SM) PSNPs and for 30, 60, and 120 min for the other PSNPs. Exposure medium was then aspirated and the cells were washed once with 100 µl/well PBS buffer at 37 °C. As the PSNPs had different fluorescent labels, two different staining protocols were used. The cells exposed to the red 50 nm (-SM) and (-CM) PSNPs were incubated with a mixture (100 µl/well) of 4 µM Hoechst (Molecular Probes®, life technologies; USA) (blue; nucleus stain) and 1 µM Calcein AM cell permeant dye (Molecular Probes®, life technologies) (green; cytoplasm). The cells exposed to the yellow 50- and 200 nm (-CP) PSNPs were incubated with a mixture (100 µl/well) of 4 µM Hoechst (blue; nucleus) and 1 µM deep red MitoTracker (Molecular Probes®, life technologies) (red; mitochondria). Cells were incubated in the dark at 37 °C, 5% CO2 for 30 min.
Cellular adhesion and uptake of PSNPs was analysed using a Cellavista™ HC imaging system (SynenTec Bio Services; Munster, Germany). This HC imaging system uses an automated, quantitative fluorescence microscope with image acquisition and software to analyse multiparameter fluorescent cellular signals to quantify the local fluorescence intensity . The output data were further processed using Microsoft Excel®2016 and Prism® 5 software. PSNP adhesion and uptake was expressed as a fluorescence intensity per cell and as a median fluorescence intensity of the entire cell population. Distribution profiles of PSNP association and uptake in a cell population were made with GraphPad Prism® 5. The number of cells correlating to each concentration bin was expressed as a percentage of the total number of exposed cells.
PSNP cellular transport
Caco-2 cells were seeded at a density of 40,000 cells/cm2 on transwell permeable PET inserts (0.4 μm pore size, 1.12 cm2 surface area, Corning®; New York, USA). Cells were maintained for 21 days (37 °C, 5% CO2) and the apical and basolateral medium was changed every other day.
The integrity of the cell barrier was monitored by measuring the transepithelial electrical resistance (TEER) values with a chopstick electrode (STX01) connected to a Millicell ERS-2 Epithelial Volt- Ohm Meter (Millipore®; USA). Inserts with TEER values of 200 Ω cm2 and higher were used in the experiments. Additionally, the transport of lucifer yellow and 4- and 10 kDa- fluorescein isothiocyanate (FITC)-dextrans (Sigma-Aldrich; USA) was analysed by measuring the fluorescence intensity in the basolateral compartment after 1 h exposure at 37 °C at 485/530 nm using a BioTek Synergy™ HT Multi-Mode Microplate reader. Control samples received EGTA (Sigma-Aldrich) for 1 h at 37 °C to induce leakage of the cellular barrier (data not shown).
PSNPs exposure media were prepared at a concentration of 250 μg/ml in DMEM+, further diluted in DMEM+ when necessary, and directly applied apically onto the cells (500 μl/insert) on day 21 of culture. After 24 h of exposure, the basolateral medium was collected and fluorescence was measured at excitation/emission wavelengths of 530/590 nm and 485/530 nm, for red and yellow-green PSNPs, respectively using a microplate reader. The results are expressed as a percentage of transported PSNP from the total nominal dose of exposure. All experiments were conducted in triplicate.
For confocal microscopy, 1.5 × 104 cells/cm2 were seeded into 8 well µ-Slides (Ibidi®; Martinsried, Germany) and incubated at 37 °C, 5% CO2 for 24 h. Afterwards, medium was discarded and cells were fixed with 200 µl/well of 4% paraformaldehyde for 15 min at room temperature. The fixation solution was discarded and cells were washed three times with 400 µl of PBS for 2–5 min, which was then replaced by 200 µl/well of permeabilization solution (FIX & PERM® Cell Fixation & Cell Permeabilization Kit, life Technologies). After 15 min incubation at room temperature the cells were washed three times with 400 µl PBS for 2–5 min and incubated for 30 min at room temperature with 400 µl/well blocking buffer (1% BSA in PBS). The blocking buffer was discarded and 100 µl of LAMP-1 mouse primary antibody (a lysosomal marker) was added to the cells and incubated for 60 min at room temperature. Cells were washed three times with 100 µl PBS and 100 µl/well of the secondary antibody (Alexa Fluor 488 for cells exposed to the red PSNPs or Alexa Fluor 594 for cells exposed to the yellow PSNPs) added and incubated with the cells for 30 min at room temperature in the dark. The samples were then washed three times with PBS before addition of 100 µl/well of DAPI (Molecular Probes®, life technologies) which was incubated for 10 min at room temperature in the dark. Samples were washed three times with PBS and cells were stored in PBS 200 µl/well in the dark until analysis. The cells were analysed using a confocal laser scanning microscope (LSM 510-META, Zeiss, Germany) using 405, 488, and 543 nm lasers and the following filters for emission; BP420-480, BP505-530, and LP615.
Characterization/quantification of protein corona of NPs
PSNPs protein corona collection
All 50 nm PSNPs at a concentration of 1 mg/ml and an equal total surface area of 200 nm PSNP were incubated in DMEM+ for 10, 20, 30, 60, 120 min at 37 °C. Afterwards, the samples were centrifuged (Hettich; Tuttlingen, Germany) for 40 min at 18,000g/15 °C. The pellets were three times re-suspended in 1 ml PBS and centrifuged for 25 min at 18,000g/4 °C. Laemmli loading buffer (Biorad—USA) containing β-mercaptoethanol was used to re-suspend the final pellet before boiling for 5 min at 95 °C followed by short centrifugation.
The total protein content in the samples was measured with a RC-DC Protein Assay (BIO-RAD) according to the manufacturer recommended protocol. All experiments were conducted in triplicate. DMEM+ was included as a control.
One dimensional sodium-dodecyl polyacrylamide gel-electrophoresis (1D - SDS-PAGE)
The required amount of protein (8 µg/well) was loaded onto pre-cast 12% SDS-PAGE gels of 1 mm thickness (BIO-RAD). 1D gel electrophoresis was then performed at 90 V for about 80 min. A protein ladder of 10–250 kDa was included in each gel. The gels were washed once with MQ water then with a water-based solution of 40% ethanol and 10% acetic acid for 15 min. Subsequently, the gels were stained overnight with Colloidal Coomassie Stain G-250 (BIO-RAD) on a rotating plate. After de-staining, the gels were scanned and the density of the bands was determined using an Odyssey scanner (Li-Cor ISO 9001, Odyssey Biosciences, Bad Homburg, Germany).
On-beads digestion—as described in —and µColumn (C18) cleaning procedures were applied to the protein corona samples before measurement by reversed-phase nano LC–MS/MS. Briefly, 18 μl of the collected protein corona samples of all PSNPs incubated in DMEM+ for 10, and 30 min at 37 °C were injected onto a Magic C18AQ 200A 5 µm beads (Bruker, USA) pre-concentration column (prepared in house) using a vacuum pump at a maximum pressure of 270 bar. Peptides were eluted and then injected into a 0.10 × 250 mm Magic C18AQ 200A 3 µm beads analytical column (prepared in-house) and eluted using an acetonitrile gradient at a flow of 0.5 μl/min with a Proxeon EASY nanoLC (Thermo Fisher Scientific, Waltham, MA, USA). The 1 h gradient consisted of an increase from 8 to 33% acetonitrile in water with 5 ml/l acetic acid in 50 min, followed by a fast increase up to 80% acetonitrile in water and 5 ml/l acetic acid (in both the acetonitrile and the water) in 3 min as a column cleaning step. Following, an electrospray potential of 3.5 kV was applied.
Full scan positive mode fourier transform mass analysers (FTMS) spectra were measured between m/z 380 and 1400 on a LTQ-Orbitrap XL (Thermo electron, San Jose, CA, USA) at high resolution (60,000). Tandem mass spectrometry (MS/MS) scans of the four most abundant 2 and 3 + charged peaks in the FTMS scan were recorded in a data dependent mode in the linear trap. LCMS runs with all MS/MS spectra obtained were analysed with MaxQuant 18.104.22.168 [27, 28].
The concentrations of the identified proteins from the PSNP coronas were determined using MassPREP tryptically digested standards (Water; Milford, USA). Standards contained a mixture of yeast enolase (SwissProt P00924), phosphorylase b (SwissProt P00489), bovine haemoglobin (SwissProt HBA P01966, HBB P02081), yeast alcohol dehydrogenase (ADH, SwissProt P00330) and bovine serum albumin (BSA, SwissProt P02769) dissolved into a range of concentrations between 0.5 and 8 pmol in 1 ml/l formic acid. Before analysis on the LC–MS/MS, 5 µl of each concentration of each standard was mixed with a sample of all NPs. This sample consisted of protein coronas isolated from equal amounts of all PSNPs used in this study after the digestion and cleaning up procedures—in a final volume of 50 µl in 1 ml/l formic acid.
Data processing and analysis
To quantitatively identify the proteins in the PSNP coronas a bovine database downloaded from Uniprot (release July 2016) (http://www.uniprot.org, 20.343 entries) , as well as a small database containing the four internal standard proteins were used together with a contaminants database that contains sequences of common contaminants like Trypsins (P00760, bovine and P00761, porcine) and human keratins (Keratin K22E (P35908), Keratin K1C9 (P35527), Keratin K2C1 (P04264) and Keratin K1CI (P35527)) . The “label-free quantification” options were enabled and the MaxQuant protein Groups output file was filtered stringently by accepting only peptides and proteins with a false discovery rate (FDR) of less than 1% and proteins with at least two identified peptides of which at least one should be unique and at least one should be unmodified.
From the set of proteins standards, iBAQ intensities of phosphorylase b (SwissProt P00489) were selected for quantification of all proteins identified in the PSNP corona and DMEM+ samples. Identified proteins were grouped based on their biological function using the aforementioned Uniprot database . The mass of each group was expressed as a percentage of the total mass of proteins and as number of molecules per cm2 (total copy number).
Each data point represents the average of three independent experiments (n = 3) and the results are shown as a mean ± standard deviation after analysis by Prism® (v.5.0; GraphPad®, USA) software. A one-way analysis of variance (ANOVA) with a Tukey’s post-test was used to test statistical significance after testing the normality distribution of the data sets using Kolmogorov–Smirnov test. A P-value < 0.05 was considered significant.
Physicochemical characterization of the PSNPs
To characterize and assess the stability of the PSNP suspensions, the hydrodynamic diameters (dh) and zeta-potentials (ζ-potential) were measured in DMEM+ at the same incubation times used in the experiments. Compared to the samples in water among all PSNPs tested, only the 50 and 200 nm (-CP) showed a significant increase in size upon incubation in DMEM+, while the incubation time showed a significant influence only on the size of 200 nm (-CP). The ζ-potentials of all the PSNPs suspended in DMEM+ were similar and stable during 24 h incubation (Table 1).
Cytotoxicity experiments (WST-1 assay) were performed to derive non-toxic concentrations of PSNPs for the uptake studies. Results demonstrated that after 3 h and 24 h exposure the cellular viability of Caco-2 cells was not affected (viability was always higher than 85% and 80% after 3 h and 24 h, respectively, compared to controls) in any of the concentrations tested (Fig. 1a, b).
Cellular adhesion and uptake of PSNPs
Cellular association of PSNPs was quantified using HC imaging analysis. The HC images are taken from above the cells, thereby merging the fluorescent signal of both internalized and membrane adhered PSNPs into one image. PSNP internalization in Caco-2 cells was therefore confirmed using confocal microscopy (Fig. 2). The PSNPs partially co-localized with lysosomes after 24 h exposure indicating (partial) internalization of the PSNPs in the lysosomes.
PSNP adhesion and cellular uptake was measured on a cell-per-cell basis using an HC imaging system during 10–120 min exposure to concentrations ranging between 15 and 250 µg/ml and expressed as median fluorescence intensity per cell. The cellular adhesion and uptake of the 50 nm (-SM) PSNPs by Caco-2 cells was, at all time-points, significantly higher compared to the 50 nm (-CM), (-CP) and 200 nm (-CP) PSNPs (Fig. 3a). Cellular distribution profiles show that cellular association with the PSNPs increased upon increasing the PSNP concentration, seen as a right shift of the median in the adhesion and uptake distribution curves (Fig. 3b). The graph also shows that at concentrations of 75 µg/ml and higher part of cell population have fluorescence signals that reached or exceeded the maximum detection limit of the HC imaging system. For all PSNPs cellular adhesion and uptake increased with increasing concentration (Fig. 3c). At the higher concentrations the increase of cellular adhesion/uptake declines and stops, which is most likely due to the detection limit of the system. For the PSNPs that associated to the largest extent with the cells, namely the 50 nm (-SM) PSNPs, the cellular adhesion and uptake distribution profile over the entire cell population was further analysed (Fig. 3b) at the single cell level with is possible with HC imaging. The results obtained clearly point at an increased fluorescent signal associated with single cells with increasing dose levels. Finally, the apparent cellular adhesion and uptake of the two PSNPs with different sizes (i.e. 50 and 200 nm) but with the same surface chemistry, was not significantly different at all concentrations and time points tested (Fig. 3c). However, the ISDD model output (Table 1) that indicates a 1.4 fold lower fraction deposited of the 200 nm (-CP) PSNPs at 30 min compared with the 50 nm PSNPs with the same surface chemistry. The apparent cellular adhesion and uptake is comparable for both PSNPs. After correction of the lower deposition of the 200 nm (-CP) PSNPs the cellular adhesion and uptake of the 200 nm (-CP) PSNPs at 30 min is 1.4 fold higher for the 200 nm (-CP) compared with the 50 nm (-CP) PSNPs with the same surface chemistry.
Transport of PSNPs across a monolayer of Caco-2 cells
To assess if cellular adhesion and uptake of PSNPs is predictive for transport across a monolayer of Caco-2 cells we performed additional experiments. A differentiated monolayer of Caco-2 cells was exposed to 250 µg/ml of each of the four PSNPs for 24 h. The longer exposure of 24 h was required to reach detectable concentration in the apical compartment of the transwell system. The transport markers used including the lucifer yellow and dextrans showed very minimal transport through Caco-2 monolayers and upon the application of EGTA to open the tight junctions, the permeability of these monolayers increased significantly (data not shown), indicating the functionality of tight junction integrity of the monolayers used in the transport studies [9, 30]. Transport of the PSNPs was determined by PSNP fluorescence measurement in the basolateral medium post exposure and expressed as a percentage of the amount of PSNP fluorescence in the medium that was applied apically at the start of the experiment (Fig. 4). The 50 nm (-SM) PSNPs showed the highest transport among all PSNPs tested (13.9%; p < 0.05), followed by the 50 nm (-CP) PSNPs (2.82%; p < 0.05). While the transport of the other carboxylated PSNPs—50 nm (-CM) and 200 nm (-CP)—did not show significant transport to the basolateral compartment (< 1%). However, if the 1.6 fold lower deposited PSNPs fraction after 24 h incubation of the PSNPs is taken into account (Table 1), the amount of the 200 nm (-CP) PSNPs is comparable to the transported amount of the 50 nm PSNPs with the same surface chemistry. Here we assume that the transport of the PSNPs increases with the concentration at the cell surface as shown for the cellular adhesion and uptake (Fig. 3).
Characterization of PSNPs protein corona
All PSNPs were incubated in DMEM+ at 37 °C for 10 and 30 min. The protein corona was then collected and analysed using SDS-PAGE. The gel was loaded with the same amount of protein for all tested PSNPs. The gels did not show large differences between the different PSNPs nor between the 10 and 30 min incubation time (Additional file 1: Figure S1). Furthermore, the protein corona was quantified and characterized using label-free nano-LC/MS–MS, which resulted in approximately 172 different adsorbed proteins. The complete list of identified proteins is provided in Additional file 2: Table S1. Proteins were clustered into 6 classes according to their biological function (and 1 “other” group). Comparing the relative amount (i.e. abundance) of a protein class on each nanoparticle to the protein class distribution as present in the cell culture medium, we observed an enrichment of proteins involved in binding, apolipoproteins, and acute phase proteins and a less pronounced enrichment of coagulation and complement factors (Fig. 5a). Subsequently, the total number of protein molecules per particle was calculated. On a single 50 nm PSNP around 2200–4000 protein molecules were absorbed (with the number of proteins on the different types of 50 nm PSNPs not being significantly different), while on the 200 nm PSNP about 59,000 proteins were absorbed (Fig. 5b). The number of proteins per surface area is between 3 × 1013 and 5 × 1013 proteins per cm2 for the 50 nm while it is about 6 × 1013 proteins per cm2 for the 200 nm PSNPs. Comparable or slightly more proteins are absorbed per cm2 on the 200 nm sized PSNP compared to the 50 nm PSNPs, an observation that might be explained by less steric hindrance on the larger particles. Among the top 20 most abundant proteins in the coronas of the 4 PSNPs, the protein Alpha-1B-glycoprotein (A1BG) ranked highest (Fig. 5c). More detailed statistical evaluation of the protein concentration on a single protein level in the coronas of the three different 50 nm PSNPs demonstrated differences in Alpha-2-macroglobulin (A2M), Alpha-fetoprotein (AFP), Apolipoprotein A-II (APOA2), Beta-2-glycoprotein 1 (APOH), and Hemoglobin fetal subunit beta (LOC781674 or HBB). Corona concentrations of most of these proteins we lower in the corona’s of the 50 nm (-SM) PSNPs, this was reaching significance only compared to the (-CM) PSNPs for the A2 M, AFP and HBB, while compared to both (-CM) and (-CP), the concentrations proteins APOA2 and APOH were lower in the corona’s of (-SM) (Fig. 6). For this evaluation only proteins with two or more copy numbers on at least one of the three different PSNPs were considered (~ 70 proteins in total).
Here, the effects of nanoparticle (NP) size and surface chemistry on the protein corona formation and subsequent cellular association (i.e. adhesions and uptake) and transport across a monolayer of Caco-2 cells is reported. Fluorescently labelled PSNPs were selected as model particles owing to their dispersion stability in cell culture media and the commercial availability in different sizes and surface modifications.
Characterization of the PSNPs, by determining the hydrodynamic size and zeta-potential of the PSNPs in cell culture medium, showed that all 50 nm PSNP suspensions were stable during the exposure times in the experiments. The DLS method as used here has been evaluated in a inter laboratory testing project  to characterize the size of the PSNPs in water or DMEM + and it was found that the proteins present in the cell culture medium resulted in a signal indicating a hydrodynamic diameter of 27 ± 2 nm. The zeta-potential of all PSNPs in cell culture medium was comparable and stable over time, irrespective of the PSNP surface chemistry with a negative charge on the PSNPs’ surface results from the PSNPs, the proteins adsorbed on the surface of the PSNPs or from measuring protein aggregates of medium rather than PSNPs .
The absence of cytotoxic effects of all PSNP concentrations used in this study was in concordance with findings from previous studies using 50 nm PSNPs functionalized with carboxyl (-CM and -CP) and sulfone (-SM) groups, using a variety of cell models [21, 32]. Confocal microscopy imaging in different planes of the cells showed internalization of the PSNPs, and partial co-localization of the PSNPs with lysosomes after 24 h of exposure. Thereby, confirming previous studies indicating uptake of negatively charged 60 nm and 100 nm PSNPs , and 50 nm and 100 nm silica (SiO2) NPs into the lysosomes [34, 35] and localization of NPs in the cytoplasm around the nucleus (for 50 nm, 90 nm, and 100 nm PSNPs) [35,36,37,38].
The cellular fluorescence as determined by HC resulting from sulfone (-SM) functionalized PSNP associated with Caco-2 cells was significantly higher compared to cells exposed to carboxylated (-CP and -CM) PSNPs of the same size. Cellular association of all functionalized PSNPs was dose dependent. Contrary to our expectations, no linear phase in the PSNP uptake kinetics by Caco-2 cells was observed, or this happened before the first time point (10 min) assessed in this experiment. Accordingly, no uptake rates of these PSNPs could be derived. The PSNPs association kinetics as observed here could be due to two processes taking place in parallel; namely PSNP cell membrane adhesion and cellular internalization. Lesniak et al. has reported very comparable time dependent changes in cellular fluorescence intensities in A549 (carcinoma human alveolar basal epithelial cells) exposed to 40 nm PSNPs over time. It was shown that during the first 10 min of exposure, cellular adhesion of PSNPs occurs rapidly, whereas after that the adsorption grows much slower [34, 39, 40]. This confirms the fast increment in fluorescence at the cells as observed by us, in the first 10 min of exposure. Recent modelling of these processes (in A549 cells) confirmed these time lines, until 20 min after exposure the PSNPs were mainly associated with the cell membranes, while after 2–3 h exposure, the PSNPs were found close to the lysosomes located centrally in the cells . The subsequent increment in fluorescence between 60 and 120 min as we reported here, might suggest PSNP uptake by the Caco-2 cells. In addition, earlier studies using 100 nm polylactic polyglycolic acid (PLGA) NPs showed that their uptake by Caco-2 cells is taking place between 1 and 2 h of exposure .
Earlier studies focused on potential optimal size for cellular uptake. By exposing Caco-2 cells to 25, 50, 100, 200 and 500 nm PSNPs preferred uptake of 100 nm PSNPs was found using a microplate reader . Uptake of 50 nm mesoporous silica NPs by HeLa cells was higher compared to 100 nm NPs after 5 h exposure . However, in EAhy926 cells, uptake of 200 nm PSNPs was higher than 20 nm PSNPs after 24 h exposure to . Comparing our observations and the data from literature point to cell type specific differences in uptake processes [14, 45]. Here we only compared studies using NPs with a comparable (effective) density. Comparing NP uptake data between studies needs to be performed with care as the reported cellular uptake is largely dependent on the particokinetics (i.e. diffusion and sedimentation) that is affected by the effective density of NPs . Indeed when correcting the applied concentrations for the ISDD estimated deposited fraction , the cellular association/uptake of 200 nm (-CP) PSNPs becomes up to 1.4 fold higher compared to 50 nm PSNPs with the same surface chemistry, whereas without this correction the estimated uptake levels were found to be similar. Nonetheless, the surface chemistry was observed to outweigh the impact of size on the observed PSNP cellular associations with the sulfone functionalized PNPSs being higher associated to the cells than the carbonyl functionalized nanoparticles. Reported differences in NP uptake thus not always reflect differences in biological processes, but merely the physiochemical interaction of NPs with the exposure media.
The type of surface functionalization on NPs was found earlier to be one of the major factors determining adhesions, uptake, transport, and distribution of NPs, which appears to be mainly driven by the size of the protein corona [9, 46]. Here, we extended our previous semi-quantitative protein corona analysis using SDS-PAGE (Additional file 1: Figure S1) with a quantitative proteomic analysis using label-free LC–MS/MS, as described by . As previously, and commonly, done, the present study was performed in the presence of fetal bovine serum. It should be noted that different types of protein mixtures are being used for in vitro studies, which might affect the outcome and thus the comparability of studies . The proteomic analysis showed that the protein corona isolated from the PSNPs was composed of 172 different proteins. We observed an enrichment of proteins involved in binding, apolipoproteins, and acute phase proteins’ groups and a less pronounced enrichment of complement factors proteins group. Among these proteins, the alpha-1B-glycoprotein (A1BG) protein was most abundantly present on all types of NPs, but the function of this protein is currently unknown. In other studies apolipoproteins have been identified as a dominant protein group in NP protein coronas [47,48,49]. Comparing the protein corona composition among the PSNPs studied here, it was found that A2M, AFP, APOA2, APOH and HBB proteins were significantly less absorbed on the (-SM) functionalized PSNPs Strikingly, the cellular association and transport across a monolayer of Caco-2 cells of these (-SM) functionalized PSNPs was also significantly different compared to the carboxylated PSNPs. Two studies have successfully attempted to correlate the composition of the protein composition of the nanoparticle corona with cellular interaction [50, 51]. In these two correlative studies different proteins were identified to correlate with cellular association of NPs. Some of the identified apolipoproteins and A2M were also found in our study to be differently enriched in the coronas of our PSNPs. It has however proven to be difficult to identify a set of specific proteins that is directly linked (mechanistically) with cellular membrane association and subsequent NP update. Previously, using corona enrichment studies, it has been described that APOA2 and APOH interfere with the cellular uptake of NPs . Here we show that different surface chemistry of PSNPs to some extent specifically enriches some proteins, like lipoproteins, binding proteins, and acute phase proteins in the corona. Some of these proteins have been associated with differential cellular interaction. A yet unresolved question is, what effects the presence of exogenous proteins from for instance food (allergy epitopes) proteins can have on the cellular interaction, as it was found that specific food related proteins in the NP corona enhance the uptake of these NPs .
Cellular association experiments using 24 h old Caco-2 cells can be performed much faster compared to monolayer transport studies that require 21 days to differentiate Caco-2 cells. Therefore, cellular association profiles of the PSNPs studied here were compared with transported amounts of these PSNPs across a monolayer of Caco-2 cells. Both, the cellular association of the (-SM) functionalized PSNPs and transported amount of these particles were higher than for the other PSNPs. This supports the previous conclusion that the adhesion properties of NPs to the cell membrane are key determinants of NP uptake , and thus likely also predictive for NP transport and could serve as a rapid screening of the intestinal transport potential of NPs is important in a tiered risk assessment or grouping approach .
The cellular uptake of NPs is highly dependent on both the intrinsic and extrinsic properties of NPs. Based on our findings, we conclude that NP surface functionalization is a more important NP property than NP size, for the cellular association of PSNPs. The type and composition of the protein corona formed on the NP surface is affected by the physicochemical properties of the NP. The protein corona is consequently one of the major players affecting the NP cellular interactions including their cytotoxicity, membrane adhesion, uptake and transport. Further studies are required to identify the set of corona proteins that affect the uptake and transport of NPs. Membrane adhesion and cellular uptake profiles correlate with the observed transport across a monolayer of Caco-2 cells, indicating membrane adhesion studies can potentially be used to predict the transport potential of NPs.
Das M, Ansari KM, Tripathi A, Dwivedi PD. Need for safety of nanoparticles used in food industry. J Biomed Nanotechnol. 2011;7:13–4.
Peters RJB, Bouwmeester H, Gottardo S, Amenta V, Arena M, Brandhoff P, Marvin HJP, Mech A, Moniz FB, Pesudo LQ, et al. Nanomaterials for products and application in agriculture, feed and food. Trends Food Sci Technol. 2016;54:155–64.
Bouwmeester H, Brandhoff P, Marvin HJP, Weigel S, Peters RJB. State of the safety assessment and current use of nanomaterials in food and food production. Trends Food Sci Technol. 2014;40:200–10.
Hansen S, Michelson E, Kamper A, Borling P, Stuer-Lauridsen F, Baun A. Categorization framework to aid exposure assessment of nanomaterials in consumer products. Ecotoxicology. 2008;17:438–47.
Zhang J, Cai X, Zhang Y, Li X, Li W, Tian Y, Li A, Yu X, Fan C, Huang Q. Imaging cellular uptake and intracellular distribution of TiO2 nanoparticles. Anal Methods. 2013;5:6611–6.
des Rieux A, Fievez V, Garinot M, Schneider Y-J, Préat V. Nanoparticles as potential oral delivery systems of proteins and vaccines: a mechanistic approach. J Control Release. 2006;116:1–27.
Shakweh M, Ponchel G, Fattal E. Particle uptake by peyer’s patches: a pathway for drug and vaccine delivery. Expert Opin Drug Deliv. 2004;1:141–63.
Yun Y, Cho YW, Park K. Nanoparticles for oral delivery: targeted nanoparticles with peptidic ligands for oral protein delivery. Adv Drug Deliv Rev. 2013;65:822–32.
Walczak AP, Kramer E, Hendriksen PJM, Tromp P, Helsper JPFG, van der Zande M, Rietjens IMCM, Bouwmeester H. Translocation of differently sized and charged polystyrene nanoparticles in in vitro intestinal cell models of increasing complexity. Nanotoxicology. 2015;9:453–61.
Arts JHE, Hadi M, Irfan M-A, Keene AM, Kreiling R, Lyon D, Maier M, Michel K, Petry T, Sauer UG, et al. A decision-making framework for the grouping and testing of nanomaterials (DF4nanoGrouping). Regul Toxicol Pharmacol. 2015;71:S1–27.
Bhattacharjee S, Ershov D, Gucht JV, Alink GM, Rietjens IM, Zuilhof H, Marcelis AT. Surface charge-specific cytotoxicity and cellular uptake of tri-block copolymer nanoparticles. Nanotoxicology. 2013;7:71–84.
He C, Hu Y, Yin L, Tang C, Yin C. Effects of particle size and surface charge on cellular uptake and biodistribution of polymeric nanoparticles. Biomaterials. 2010;31:3657–66.
Lynch I, Weiss C, Valsami-Jones E. A strategy for grouping of nanomaterials based on key physico-chemical descriptors as a basis for safer-by-design NMs. Nano Today. 2014;9:266–70.
Ritz S, Schöttler S, Kotman N, Baier G, Musyanovych A, Kuharev J, Landfester K, Schild H, Jahn O, Tenzer S, Mailänder V. Protein corona of nanoparticles: distinct proteins regulate the cellular uptake. Biomacromolecules. 2015;16:1311–21.
Hühn D, Kantner K, Geidel C, Brandholt S, De Cock I, Soenen SJH, Rivera_Gil P, Montenegro J-M, Braeckmans K, Müllen K, et al. Polymer-coated nanoparticles interacting with proteins and cells: focusing on the sign of the net charge. ACS Nano. 2013;7:3253–63.
Kim JA, Salvati A, Aberg C, Dawson KA. Suppression of nanoparticle cytotoxicity approaching in vivo serum concentrations: limitations of in vitro testing for nanosafety. Nanoscale. 2014;6:14180–4.
Walczyk D, Bombelli FB, Monopoli MP, Lynch I, Dawson KA. What the cell “sees” in bionanoscience. J Am Chem Soc. 2010;132:5761–8.
Yin Win K, Feng S-S. Effects of particle size and surface coating on cellular uptake of polymeric nanoparticles for oral delivery of anticancer drugs. Biomaterials. 2005;26:2713–22.
Fröhlich E. The role of surface charge in cellular uptake and cytotoxicity of medical nanoparticles. Int J Nanomed. 2012;7:5577–91.
Ramery E, O’Brien PJ. Evaluation of the cytotoxicity of organic dust components on THP1 monocytes-derived macrophages using high content analysis. Environ Toxicol. 2014;29:310–9.
Anguissola S, Garry D, Salvati A, O’Brien PJ, Dawson KA. High content analysis provides mechanistic insights on the pathways of toxicity induced by amine-modified polystyrene nanoparticles. PLOS ONE. 2014;9:e108025.
Hinderliter PM, Minard KR, Orr G, Chrisler WB, Thrall BD, Pounds JG, Teeguarden JG. ISDD: a computational model of particle sedimentation, diffusion and target cell dosimetry for in vitro toxicity studies. Part Fibre Toxicol. 2010;7:36.
Fröhlich E, Bonstingl G, Höfler A, Meindl C, Leitinger G, Pieber TR, Roblegg E. Comparison of two in vitro systems to assess cellular effects of nanoparticles-containing aerosols. Toxicol In Vitro. 2013;27–360:409–17.
Elliott J, Rösslein M, Song N, Toman B, Kinsner- Ovaskainen A, Maniratanachote R, Salit M, Petersen E, Sequeira F, Romsos E, Kim S, Lee J, von Moos N, Rossi F, Hirsch C, Krug H, Suchaoin W, Wick P. Toward achieving harmonization in a nanocytotoxicity assay measurement through an interlaboratory comparison study. Altern Anim Exp. 2017;34:201–18.
Franscini N, Wuertz K, Patocchi-Tenzer I, Durner R, Boos N, Graf-Hausner U. Development of a novel automated cell isolation, expansion, and characterization platform. J Assoc Lab Autom. 2011;16:204–13.
Wendrich JR, Boeren S, Möller BK, Weijers D, De Rybel B. In vivo identification of plant protein complexes using IP-MS/MS. In: Kleine-Vehn J, Sauer M, editors. Plant hormones: methods and protocols. New York: Springer; 2017. p. 147–58.
Cox J, Mann M. MaxQuant enables high peptide identification rates, individualized p.p.b.-range mass accuracies and proteome-wide protein quantification. Nat Biotechnol. 2008;26:1367–72.
Cox J, Neuhauser N, Michalski A, Scheltema RA, Olsen JV, Mann M. Andromeda: a peptide search engine integrated into the MaxQuant environment. J Proteome Res. 2011;10:1794–805.
Consortium TU. UniProt: the universal protein knowledgebase. Nucleic Acids Res. 2017;45:D158–69.
Bouwmeester H, Poortman J, Peters RJ, Wijma E, Kramer E, Makama S, Puspitaninganindita K, Marvin HJP, Peijnenburg AACM, Hendriksen PJM. Characterization of translocation of silver nanoparticles and effects on whole-genome gene expression using an in vitro intestinal epithelium coculture model. ACS Nano. 2011;5:4091–103.
Langevin D, Lozano O, Salvati A, Kestens V, Monopoli M, Raspaud E, Mariot S, Salonen A, Thomas S, Driessen M, et al. Inter-laboratory comparison of nanoparticle size measurements using dynamic light scattering and differential centrifugal sedimentation. NanoImpact. 2018;10:97–107.
Wang F, Yu L, Monopoli MP, Sandin P, Mahon E, Salvati A, Dawson KA. The biomolecular corona is retained during nanoparticle uptake and protects the cells from the damage induced by cationic nanoparticles until degraded in the lysosomes. Nanomed Nanotechnol Biol Med. 2013;9:1159–68.
Åberg C, Varela JA, Fitzpatrick LW, Dawson KA. Spatial and structural metrics for living cells inspired by statistical mechanics. Sci Rep. 2016;6:34457.
Shapero K, Fenaroli F, Lynch I, Cottell DC, Salvati A, Dawson KA. Time and space resolved uptake study of silica nanoparticles by human cells. Mol BioSyst. 2011;7:371–8.
Xia T, Kovochich M, Liong M, Zink JI, Nel AE. Cationic polystyrene nanosphere toxicity depends on cell-specific endocytic and mitochondrial injury pathways. ACS Nano. 2008;2:85–96.
Yacobi NR, DeMaio L, Xie J, Hamm-Alvarez SF, Borok Z, Kim K-J, Crandall ED. Polystyrene nanoparticle trafficking across alveolar epithelium. Nanomed Nanotechnol Biol Med. 2008;4:139–45.
Hemmerich PH, von Mikecz AH. Defining the subcellular interface of nanoparticles by live-cell imaging. PLoS ONE. 2013;8:e62018.
Bhattacharjee S, Ershov D, Fytianos K, van der Gucht J, Alink GM, Rietjens IMCM, Marcelis ATM, Zuilhof H. Cytotoxicity and cellular uptake of tri-block copolymer nanoparticles with different size and surface characteristics. Part Fibre Toxicol. 2012;9:1–19.
Salvati A, Åberg C, dos Santos T, Varela J, Pinto P, Lynch I, Dawson KA. Experimental and theoretical comparison of intracellular import of polymeric nanoparticles and small molecules: toward models of uptake kinetics. Nanomed Nanotechnol Biol Med. 2011;7:818–26.
Lesniak A, Salvati A, Santos-Martinez MJ, Radomski MW, Dawson KA, Åberg C. Nanoparticle adhesion to the cell membrane and its effect on nanoparticle uptake efficiency. J Am Chem Soc. 2013;135:1438–44.
Desai MP, Labhasetwar V, Walter E, Levy RJ, Amidon GL. The mechanism of uptake of biodegradable microparticles in caco-2 cells is size dependent. Pharm Res. 1997;14:1568–73.
Kulkarni SA, Feng S-S. Effects of particle size and surface modification on cellular uptake and biodistribution of polymeric nanoparticles for drug delivery. Pharm Res. 2013;30:2512–22.
Lu F, Wu S-H, Hung Y, Mou C-Y. Size effect on cell uptake in well-suspended, uniform mesoporous silica nanoparticles. Small. 2009;5:1408–13.
Fröhlich E, Meindl C, Roblegg E, Ebner B, Absenger M, Pieber TR. Action of polystyrene nanoparticles of different sizes on lysosomal function and integrity. Part Fibre Toxicol. 2012;9:26.
Baumann D, Hofmann D, ven Nullmeier S, Panther P, Dietze C, Musyanovych A, Ritz S, Landfester K, Mailänder V. Complex encounters: nanoparticles in whole blood and their uptake into different types of white blood cells. Nanomedicine. 2013;8:699–713.
Liu J, Legros S, Ma G, Veinot JGC, von der Kammer F, Hofmann T. Influence of surface functionalization and particle size on the aggregation kinetics of engineered nanoparticles. Chemosphere. 2012;87:918–24.
Tenzer S, Docter D, Kuharev J, Musyanovych A, Fetz V, Hecht R, Schlenk F, Fischer D, Kiouptsi K, Reinhardt C, Landfester K, Schild H, Maskos M, Knauer SK, Stauber RH. Rapid formation of plasma protein corona critically affects nanoparticle pathophysiology. Nat Nanotechnol. 2013;8:772–81.
Lundqvist M, Stigler J, Elia G, Lynch I, Cedervall T, Dawson KA. Nanoparticle size and surface properties determine the protein corona with possible implications for biological impacts. Proc Natl Acad Sci USA. 2008;105:14265–70.
Cedervall T, Lynch I, Lindman S, Berggård T, Thulin E, Nilsson H, Dawson KA, Linse S. Understanding the nanoparticle–protein corona using methods to quantify exchange rates and affinities of proteins for nanoparticles. Proc Natl Acad Sci. 2007;104:2050–5.
Walkey CD, Olsen JB, Song F, Liu R, Guo H, Olsen DWH, Cohen Y, Emili A, Chan WCW. Protein corona fingerprinting predicts the cellular interaction of gold and silver nanoparticles. ACS Nano. 2014;8:2439–55.
Liu R, Jiang W, Walkey CD, Chan WCW, Cohen Y. Prediction of nanoparticles-cell association based on corona proteins and physicochemical properties. Nanoscale. 2015;7:9664–75.
Di Silvio D, Rigby N, Bajka B, Mackie A, Baldelli Bombelli F. Effect of protein corona magnetite nanoparticles derived from bread in vitro digestion on Caco-2 cells morphology and uptake. Int J Biochem Cell Biol. 2016;75:212–22.
Wrote paper, designed and performed the biological experiments: AA. Characterized the nanoparticles: AA. Proteomics analysis: AA, SB, MvdZ and JV. Confocal microscopy: AA, MvdZ and RH. High content imaging data analysis: AA, MvdZ and AP. Critically reviewed manuscript: HB, MvdZ, AP, and IR. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
Availability of data and materials
All data generated or analysed during this study are included in this published article and its additional files.
Consent for publication
Ethics approval and consent to participate
This work was supported by a NFP grant to AA, and by the Dutch department of Economic affairs to MvdZ, RH, and HB.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Additional file 1: Figure S1.
SDS-PAGE showing the protein corona of PSNPs.
Additional file 2: Table S1.
The list of identified PSNPs corona proteins using LC-MS/MS after 10 and/or 30 min incubation in DMEM+.
Rights and permissions
Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
About this article
Cite this article
Abdelkhaliq, A., van der Zande, M., Punt, A. et al. Impact of nanoparticle surface functionalization on the protein corona and cellular adhesion, uptake and transport. J Nanobiotechnol 16, 70 (2018). https://doi.org/10.1186/s12951-018-0394-6
- High throughput screening
- Cellular adhesion and uptake
- Label-free LC–MS/MS
- Quantitative proteomics