- Open Access
Changes of physico-chemical properties of nano-biomaterials by digestion fluids affect the physiological properties of epithelial intestinal cells and barrier models
Particle and Fibre Toxicology volume 19, Article number: 49 (2022)
The widespread use of nano-biomaterials (NBMs) has increased the chance of human exposure. Although ingestion is one of the major routes of exposure to NBMs, it is not thoroughly studied to date. NBMs are expected to be dramatically modified following the transit into the oral-gastric-intestinal (OGI) tract. How these transformations affect their interaction with intestinal cells is still poorly understood. NBMs of different chemical nature—lipid-surfactant nanoparticles (LSNPs), carbon nanoparticles (CNPs), surface modified Fe3O4 nanoparticles (FNPs) and hydroxyapatite nanoparticles (HNPs)—were treated in a simulated human digestive system (SHDS) and then characterised. The biological effects of SHDS-treated and untreated NBMs were evaluated on primary (HCoEpiC) and immortalised (Caco-2, HCT116) epithelial intestinal cells and on an intestinal barrier model.
The application of the in vitro SDHS modified the biocompatibility of NBMs on gastrointestinal cells. The differences between SHDS-treated and untreated NBMs could be attributed to the irreversible modification of the NBMs in the SHDS. Aggregation was detected for all NBMs regardless of their chemical nature, while pH- or enzyme-mediated partial degradation was detected for hydroxyapatite or polymer-coated iron oxide nanoparticles and lipid nanoparticles, respectively. The formation of a bio-corona, which contains proteases, was also demonstrated on all the analysed NBMs. In viability assays, undifferentiated primary cells were more sensitive than immortalised cells to digested NBMs, but neither pristine nor treated NBMs affected the intestinal barrier viability and permeability. SHDS-treated NBMs up-regulated the tight junction genes (claudin 3 and 5, occludin, zonula occludens 1) in intestinal barrier, with different patterns between each NBM, and increase the expression of both pro- and anti-inflammatory cytokines (IL-1β, TNF-α, IL-22, IL-10). Notably, none of these NBMs showed any significant genotoxic effect.
Overall, the results add a piece of evidence on the importance of applying validated in vitro SHDS models for the assessment of NBM intestinal toxicity/biocompatibility. We propose the association of chemical and microscopic characterization, SHDS and in vitro tests on both immortalised and primary cells as a robust screening pipeline useful to monitor the changes in the physico-chemical properties of ingested NBMs and their effects on intestinal cells.
In the last few years, nano-biomaterials (NBMs) have been widely used for manufacturing innovative food packaging [1, 2] nutraceuticals , cosmetics [4, 5], as well as in dentistry , precision medicine [7,8,9] and agriculture [10, 11], increasing the likelihood of human exposure through ingestion and transit through the gastro-intestinal (GI) tract .
A growing number of studies suggested a possible interference of ingested NBMs with the gut microenvironment . The human digestive apparatus is composed of many sections with different structures and functions. The most complex part is the intestinal tract. In particular, the small intestine mediates the absorption of nutrients through transcellular processes or paracellular diffusion. The latter is limited by the presence of tight junction (TJs) complexes, formed by zonula occludens-1, occludin and claudin proteins . In physiological conditions, TJs prevent water and electrolyte leakage and avoid lumen infections. However, some conditions, such as inflammatory bowel disease [15, 16], can alter the structure of TJs, increasing the intestinal barrier permeability. Two studies report that nanometric SiO2 or TiO2 can induce similar effects [17, 18].
While a substantial amount of knowledge has been accumulated for the inhalation route, only recently the fate of the ingested NBMs has gained interest in the nanotoxicology community . The poor awareness of ingestion’s relevance as exposure route to NBMs, the non-suitability of the available models, and the lack of consensus on the most suitable in vitro models reproducing the complexity of the Oral-Gastro-Intestinal (OGI) tract are the main reasons for this delay.
In the last few years, some models to mimic the intestinal barrier in vitro and study the toxicity of NBM have been proposed, as co-cultures of different intestinal cell types. Co-culture monolayers, composed by enterocyte-like cells with TJs and brush border (Caco-2), and goblet cells secreting mucus (HT29-MTX), have been used to investigate the toxicity of NBMs such as TiO2 nanoparticles [20,21,22,23] and multi walled carbon nanotubes . The effect of halloysite clay nanotube on intestinal barrier  has been also studied on Caco-2/HT29-MTX co-culture plus Raji B cells (that promote Caco-2 differentiation into M cells, characterised by the typical digestive function of enterocytes). The results have indicated the absence of cytotoxicity despite the high production of pro-inflammatory cytokines and the increase in cell growth and proliferation .
Recently, newly intestinal mucosa 3D models have been developed culturing Caco-2 cells on a layer of macrophages and dendritic cells embedded in collagen scaffolds. Indeed, these immune cells are both present in the intestinal lamina propria and react to inflammatory stimuli, by producing pro-inflammatory cytokines (e.g. interleukin (IL)-6, tumour necrosis factor (TNF)-α) and anti-inflammatory mediator (e.g. IL-10) [27, 28], as a possible compensation mechanism. Interestingly, some of these mediators such as IL-6 and TNF-α are involved in the pathogenesis of inflammatory bowel disease, promoting gut damage and loss of intestinal barrier integrity, while IL-10 reduces the inflammation typically associated with this pathology . Some NBMs have been shown to induce intestinal cells to assume the phenotype of inflammatory bowel disease. For instance, the model proposed by Susewind and co-workers to assess the safety of TiO2, Ag and Au nanoparticles  is characterised by the loss of barrier function and the increased production of inflammatory cytokines that regress after the treatment with anti-inflammatory drugs , well recapitulating the situation occurring in vivo.
Furthermore, some authors proposed ex-vivo systems derived from murine, porcine, or human bowel to study the intestinal permeability after the exposure to nanoparticles [32, 33].
Although these models are closer to the intestinal anatomy and physiology than conventional monocultures, the most used model for the evaluation of the exposure to NBMs is still the culture of Caco-2 cells on porous membrane inserts. In these conditions the cells rapidly differentiate into an intestinal barrier [34,35,36,37]. In addition the HCT116 model, another colon cancer cell line, is a widely accepted tool to evaluate the genotoxicity of NBMs [38,39,40,41].
Another important issue to be considered in in vitro intestinal models is the biological identity of the NBMs that are in contact with cells, because ingested NBMs interact with different fluids characterised by specific pH, ionic strength, and composition. This interaction may dramatically modify NBMs’ properties. For instance, the exposure may lead to dissolution , aggregation/agglomeration , and formation of bio-molecular corona  that may change over time. Monitoring such biotransformations is crucial to understand the NBMs biological fate in the gut environment and the impact on their toxicity [19, 45].
Recently, several in vitro digestion models have been proposed to investigate the digestion-driven modifications of NBMs. Sequential incubations in simulated gastric and intestinal fluids have been used to study the bioactivity of starch nanocapsules  and zein-pectin nanoparticles . A similar protocol, improved with longer incubation times and the addition of simulated saliva, has been set up to study the dissolution of Fe2O3 nanoparticles , the agglomeration of TiO2 nanoparticles and their interaction with proteins . Several other models have been proposed, differing in fluid composition or incubation times, such as the simulated digestion system reported in Sohal et al.  and slightly modified by Marucco et al. . Most of these models have been used to describe the transformation occurring to NBMs during the digestive process. Nevertheless, few studies have been published on the effects that such changes have on intestinal cells [51,52,53,54].
To fill this gap, in this study we adopted a simulated human digestion system (SHDS) consisting of sequential incubations in simulated saliva fluid (SSF), simulated gastric fluid (SGF) and simulated intestinal fluid (SIF) to investigate the biotransformation of NBMs of different chemical nature. Samples representative of NBMs with potential applications in oral drug delivery or nutraceutical field have been selected, i.e. hydroxyapatite, carbon nanoparticles, lipid-surfactant nanoparticles and surface modified magnetite nanoparticles [55,56,57,58]. The effects of SHDS-treated or untreated NBMs on viability, barrier integrity and intracellular inflammation were evaluated on primary and immortalised epithelial intestinal cells.
Properties of the NBMs
In this study, we selected the following NBMs: three colloidal formulations composed by elemental carbon nanoparticles (CNPs), lipid-surfactant nanoparticles (LSNPs) and PLGA-PEG coated magnetite nanoparticles (FNPs), and one powder sample of hydroxyapatite nanoparticles (HNPs).
The main properties of the materials are summarized in Table 1.
The size distribution and the surface properties of the NBMs were investigated by Dynamic Light Scattering (DLS) and Electrophoretic Light Scattering (ELS), respectively (Table 1 and Fig. 1A and B).
Because of the presence of particles/aggregates larger than the upper limit of detection of the DLS technique (5 µm), LSNPs and HNPs were also analysed by flow particle imaging analysis (FPIA) (size range 1–150 µm) (Fig. 1C and D).
Based on the low polydispersity index (PDI) values and on the small standard deviation (SD) of the size distribution (Table 1), CNPs and FNPs appeared stable and monodisperse colloidal suspensions. CNPs and FNPs were mainly composed of nanometric particles (< 100 nm), albeit particles/agglomerates or aggregates in the nanometric/sub-micrometric range were detected as well (Fig. 1A). According to DLS, LSNPs had a larger size than CNPs and FNPs, mainly in the sub-micrometric range (Fig. 1A). However, it might correspond to the presence of few sub-micrometric particles, since DLS techniques overestimate the abundance of particles with larger sizes. FPIA confirms the presence of few particles with a diameter between 1 and 10 μm (Fig. 1C). As far as HNPs are concerned, particles were distributed in a wide range of sizes, from 400 nm to 20 μm (Fig. 1D). In water HNPs formed unstable suspensions, with clear sedimentation during time. More details on the structure of the four NBMs were provided by transmission electron microscope (TEM) analysis (following section). As expected, LSNPs and CNPs exhibited negative ζ-potential values in the whole pH range (Fig. 1B), suggesting the presence of negatively charged surface groups. FNPs showed positive ζ-potential values only at very low pH values (Fig. 1B), likely because of the contribution of the magnetite core. HNPs had ζ-potential values close to 0 mV at all pH (Fig. 1B) that well agree with the instability of the suspensions.
Effect of the simulated human digestive system (SHDS) on the measured particles size
The transformation of the NBMs was monitored in terms of changes in size distribution, surface modifications, and degradation or dissolution by enzymatic digestion.
The changes in size distribution of NBMs during the SHDS treatment were firstly measured by integrating DLS and FPIA data. In Fig. 2 the hydrodynamic distribution in the different compartments was compared with those measured in water.
No changes of size distribution were found for LSNPs and CNPs in SSF (Fig. 2A and B), while a shift of the distribution curve toward higher diameters was observed for FNPs (Fig. 2C), suggesting agglomeration/aggregation. In the SGF a clear destabilization of the colloidal suspensions was observed for all NBMs, as inferred by the diameters shift towards high values and the increase in the standard deviation among the measurements (Fig. 2A–D). This was expected, because of the low pH and high ionic strength of the media. Because of the intrinsic instability of HNPs suspension, the effect of the SGF was less evident (Fig. 2D). The suspensions remained highly unstable also in the SIF and the presence of large aggregates was optically visible in the final suspension (Additional file 1: Fig S1). The presence of micrometric particles/aggregates or agglomerates was evaluated by FPIA (Fig. 2E–H). Micrometric particles were detected in all cases, albeit in different amounts. LSNPs (Fig. 2E) exhibited a concentration of micrometric particles higher than the untreated material, while for HNPs (Fig. 2H) a decrease was observed.
The size distribution was also measured by incubating the NBMs directly in the intestinal fluid (Additional file 1: Fig S2). In this case, the suspension appeared more stable and less aggregated than after the SHDS, suggesting that the aggregation occurred in the SGF, and was irreversible for all NBMs.
TEM analysis of the SHDS-treated and untreated NBMs was also performed (Fig. 3).
Untreated LSNPs (Fig. 3A) were composed by quasi-spherical particles of different size, confirming the DLS analysis (Fig. 1A). SHDS-treated LSNPs (Fig. 3A′) appeared of smaller dimensions, suggesting degradation, but organized in large aggregates surrounded by biological material deriving from the SHDS fluids.
Untreated CNPs (Fig. 3B) appeared spherical, well dispersed, and had a narrow size distribution around 120 nm, in agreement with the DLS data, whereas the SHDS-treated CNPs (Fig. 3B′) resulted in an agglomerated and entangled state with associated biological material, similarly to LSNPs (Fig. 3A′).
Untreated FNPs (Fig. 3C) appeared as small spherical iron oxide particles embedded inside the PLGA-PEG polymer matrix. After the SHDS (Fig. 3C′) the polymer matrix was apparently removed, likely because of the biodegradable nature of the PLGA polymer . Transparent spherical structures, which can be attributed to the polymeric residues still present after a partial biodegradation or to the biological matrix, were visible. Iron oxide particles appeared highly aggregated, because of the degradation of the polymeric matrix, in line with the results obtained by the DLS analyses (Fig. 2C). No significant alterations of the iron oxide particles morphology were observed.
Large particles of very different shapes such as rods, rectangles or spheres were observed for HNPs (Fig. 3D). This shape/size diversity can justify the instability of the colloidal suspensions and the inconclusive results in the DLS analysis. Nevertheless, SHDS-treated HNPs (Fig. 3D′) apparently underwent a dramatic transformation in terms of morphology with evident biological material surrounding the HNPs. Being soluble at acidic pH (Additional file 1: Fig S3) HNPs are expected to dissolve in the SGF , and eventually re-precipitate in the SIF.
On the other hand, LSNPs were likely subjected to hydrolysis by lipases . To investigate the susceptibility of LSNPs to enzymatic degradation, this NBM was incubated in a solution of lipase in water at the same pH as the intestinal fluid, and the size distribution was monitored up to 24 h (Additional file 1: Fig S4). A shift of the dH distribution towards lower values was observed already after 15 min (Additional file 1: Fig S4A) indicating degradation; a decrease of approximately 8% in the mean dH value occurred after 24 h (Additional file 1: Fig S4B). These data confirm the partial degradation of LSNPs observed by TEM analysis (Fig. 3A′).
Bio-molecular corona formation during SHDS
The formation of a bio-molecular corona was investigated on CNPs and FNPs, because these NBMs exhibit a surface reactivity that can be used as a probe to monitor the extent of coverage of the surface.
The SHDS was performed firstly with and without active components (proteins, bile and uric acid, Table 4), and the size distribution changes were monitored (Fig. 4).
In both SGF and SIF a higher Z-average and PDI values in the absence of active components was observed compared to fluids with active components. The suspensions were largely unstable, and the particles slowly deposited on the bottom of the flask, as shown in Fig. 4. This confirms the formation of a bio-molecular corona in the SHDS that stabilizes the colloids.
To gain information on the extent of the surface coverage, the NBMs were analysed for their surface charge by ELS and reactivity by electron paramagnetic resonance (EPR) spectroscopy (Fig. 5). The experiments were performed after washing steps aimed at removing the soft corona.
The ζ-potential was measured in ultrapure water by varying the pH of the suspension (Fig. 5A and B). The ζ-potential curves of CNPs treated with SHDS were different compared to untreated CNPs, suggesting the presence of biomolecules at the surface. Similarly, treated FNPs showed a ζ-potential shift, which might be due to the presence of a bio-molecular corona, and/or to the removal of the polymeric coating.
The surface reactivity was monitored by using the spin-probe TEMPONE-H. This is an unspecific probe able to react with Reactive Oxygen Species with redox-active surface centres leading to the stable radical TEMPONE, detectable by EPR spectroscopy . Therefore, this system is suitable to monitor the surface reactivity of nanomaterials.
In the presence of untreated CNPs (Fig. 5A′) or FNPs (Fig. 5B′), the typical three-line signal of the TEMPONE radicals was observed. When treated with SHDS the surface reactivity of both FNPs and CNPs decreased, but was not eliminated, suggesting that the surface was still partially exposed to the solvent.
NBMs identity in cell culture medium and in SHDS
In vitro cellular tests require the use of cell medium, which contains several components, including proteins. During the NBM incubation in this medium, their biological identity may be further modified due to the particles interaction with the medium components. Therefore, we firstly investigated any changes in the material size distribution following exposure to protein rich fluid. Fig 6 shows a comparison of treated and untreated NBMs diluted in cell medium (Dulbecco's Modified Eagle Medium (DMEM) with 10% Foetal Bovine Serum (FBS)). The mean dH values and PDI are reported in Additional file 1: Table S1.
The NBMs exposure to the SHDS resulted in a dramatic change of the size distribution for all NBMs.
Treated LSNPs exposed to cell medium were more stable over time than the untreated ones (Fig. 6A), but they displayed a wider range of size, with a population characterised by a mean diameter smaller than the LSNPs in water, likely as a consequence of a partial degradation. Both treated and untreated CNPs were stable in cell medium up to 24 h (Fig. 6B). A moderate shift of the sizes towards values higher than the particles in water was however observed, more evident for the treated CNPs. A visible time-dependent instability in cell medium was observed for both treated and untreated FNPs (Fig. 6C) and HNPs (Fig. 6D). Treated FNPs were largely aggregated in cell medium, while a moderate shift of the curve towards higher dH was observed for the untreated FNPs in comparison to water. Untreated HNPs appeared to form slightly more stable colloids in cell medium than in water; while after SHDS several populations with a wide range of size appeared. The formation of aggregates of size above the detection limit of DLS was clearly visible for all NBMs in cell medium (Additional file 1: Fig S5).
The surface reactivity of CNPs and FNPs in the cell medium was also monitored by EPR spectroscopy (Fig. 6E and F). Both treated and untreated CNPs had similar surface reactivity in cell medium, suggesting that the surface of the particles is still exposed to the solvent. In the case of FNPs, the SHDS-treated sample exhibited an unexpectedly high surface reactivity, likely caused by the presence in the bio-molecular corona of some redox-active components.
The hard protein corona composition was also analysed for treated and untreated NBMs after incubation in cell medium. For the isolation of the corona-NBM complex, three steps of centrifugation were necessary to remove the soft corona . However, a protein background was detected for the control sample, only composed by SHDS and DMEM 10% FBS and no NBMs (Additional file 1: Fig S6E), suggesting that the digestion process and the long incubation time led to protein aggregation. Unfortunately, it was not possible to discriminate the protein corona from the background proteins that co-precipitated during the NBMs-corona isolation protocol. Thus, we studied the effect of the treatment with SHDS only for FNPs. In fact, for these NBMs a magnetic separation was used as an alternative method to remove the soft corona. In Fig. 7A the SDS-PAGE analysis of the hard corona is shown. Clearly, the treatment with SHDS affected the corona composition since treated and untreated samples had different protein patterns.
Proteomic analysis by mass spectrometry for these samples identified more than 200 proteins for the corona of both SHDS-treated and untreated FNPs (Fig. 7B).
The top 20 most abundant proteins are listed in Table 2. Label free quantification (LFQ) calculated with Perseus was used to compare the protein abundance between the two samples.
Within the top 20 most abundant proteins, some serine proteases derived from SHDS were found in the SHDS treated sample. Different chymotrypsins derived from pancreatin were also detected among the less abundant proteins (data not shown). On the other hand, proteins highly abundant in FBS , were found in the corona for both samples, in particular alpha-2-HS-glycoprotein, apolipoprotein AI and AII, bovine haemoglobin alpha and beta chain, and alpha-1-antiproteinase. This latter, alpha-1-antiproteinase, also known as alpha-1-antitrypsin, alpha-1-proteinase inhibitor or serpin A1, is an inhibitor of serine proteases. A comparison of the abundance of proteases in treated and untreated samples is shown in Additional file 1: Fig S7.
Effects of SHDS on the cytotoxicity toward epithelial intestinal Caco-2 cells, HCT116 cells and primary human colonic epithelial cells
To investigate the effect of SHDS treatment on the NBMs cytotoxicity, a dose-dependent viability assay in Caco-2 and HCT116 cells, using a dose range from 0 to 150 µg/ml was performed.
This range was chosen based on the toxicity given by the OGI fluids alone tested at the same dilutions used for NBMs. Indeed, preliminary experiments indicated that OGI fluids were not significantly toxic up to dilution corresponding to 150 µg/ml NBMs (Additional file 1: Fig S8A).
In both Caco-2 and HCT116 cells, a very low toxicity was observed for untreated LSNPs up to 100 µg/ml. However, after the treatment with SHDS a significant cytotoxicity was observed for concentrations higher than 75 µg/ml and 20 µg/ml in Caco-2 and HCT116 cells, respectively (Fig. 8A). On the contrary, neither SHDS-treated nor untreated CNPs were toxic and SHDS did not alter the profile of toxicity of this NBM in both cell lines (Fig. 8B). On Caco-2 cells, untreated FNPs displayed the highest cytotoxicity, starting at 10 µg/ml, but in contrast with the other NBMs, SHDS has a cytoprotective effect: indeed, SHDS-treated FNPs became toxic at 50 µg/ml and were significantly less toxic than untreated ones in the range 50–75 µg/ml (Fig. 8C). A similar effect of toxicity masking was observed for HNPs: indeed, untreated HNPs were toxic from 50 µg/ml, but after SHDS no toxicity was detected at all the concentrations tested. As further confirmation, SHDS-treated HNPs were significantly less cytotoxic than untreated ones (Fig. 8D). On HCT116 cells, neither untreated nor SHDS-treated FNPs and HNPs induced any significant cytotoxicity (Fig. 8C and D).
Caco-2 and HCT116 cells are widely used as models of gastrointestinal cells . However, being immortalized, they are expected to be more resistant to external stimuli. Therefore, we measured the effect of NBMs also in primary non-transformed intestinal epithelial cells (HCoEpiC). In general, all the NBMs showed toxicity at lower concentrations than on Caco-2 and HCT116 cells (Fig. 9). This finding can be partially explained by the higher sensitivity of HCoEpiC to SHDS fluids, which are toxic at a lower concentration (50 µg/ml) (Additional file 1: Fig S8B) than in immortalized cells (Additional file 1: Fig S8A). On this basis, we decided to evaluate the NBMs at a concentration range (2.5–20 µg/ml) immediately below the first toxic concentration for SHDS fluids.
The pre-incubation with SHDS increased the cytotoxicity of LSNPs and CNPs (Fig. 9A and B). We did not detect any significant cytotoxicity changes between SHDS-treated and untreated FNPs (Fig. 9C), while HNPs were the only NBM showing lower cytotoxicity after SHDS towards both Caco-2 (Fig. 8D) and HCoEpiC cells (Fig. 9D).
These data show a different behaviour on epithelial intestinal cells in relation to the nature of NBMs that can undergo different modifications during SHDS. Moreover, the choice of in vitro model to evaluate cytotoxicity is also of paramount importance, as demonstrated by the different sensitivity between Caco-2 cells, HCT116 cells and primary non-transformed cells.
The genotoxicity of NBMs was then evaluated on HCT116 cells because, although it is a cancer-derived cell line, it bears wild-type p53 contrarily to Caco-2 cells. None of the tested NBM induced any significant increase of DNA strand breaks as assessed by counting 53BP1 DNA repair foci, while the positive control, i.e., cells exposed for 24 h to 50 µM etoposide, led to a statistically significant increase of 53BP1 foci count (Additional file 1: Fig S9).
Effects of SHDS on viability and permeability of Caco-2 intestinal barrier model
Finally, we investigated the effects of NBMs on viability, permeability, and inflammation parameters in a competent model of GI barrier, i.e. the 21-day differentiated Caco-2 model.
When Caco-2 cells grow on specific inserts and reach the complete confluence, they begin to differentiate, completing the process after 21 days . This model is recognized as a valid GI barrier model, widely used in permeability assessment tests because it mimics intestinal physiology [67, 68]. Thus, we used this model to investigate the effects on cell viability and barrier permeability for all SHDS-treated and untreated NBMs. Since there are no literature data about the physiological doses in patients exposed to these NBMs but at the same time there are also no reports of severe acute toxicity, we decided to study the highest non-toxic dose of NBMs for Caco-2 undifferentiated cells, to highlight the differences in terms of toxicological properties of NBMs, before and after the simulated digestive process. Barrier-forming cells were thus incubated for 24 h at the highest non-toxic concentrations of SHDS-treated NBMs (150 µg/ml for CNPs and HNPs and 50 µg/ml for LSNPs and FNPs) (Fig. 8, left panel).
In the viability assays, neither untreated nor SHDS-treated NBMs showed toxicity (Fig. 10A). Since toxic effects of NBMs may alter barrier integrity and produce inflammation , we next evaluated integrity parameters, in terms of functional assays, TEER and TJ levels, and pro/anti-inflammatory cytokines production.
In our model, the absence of toxicity was paralleled by the absence in permeability variation, measured by the Lucifer Yellow permeability assay (Fig. 10B; Table 3). Moreover, the TEER values were always > 600 Ω*cm2 in both untreated and NBM-treated barriers (Additional file 1: Table S2).
Notably, each NBM increased one or more genes involved in TJs with a specific pattern (Fig. 11). Untreated LSNPs, FNPs and HNPs down-regulate occludin (OCLN) (Fig. 11B) and to a lesser extent zonula occludens-1 (TJP1) (Fig. 11A), claudin 3 (CLDN3) (Fig. 11C) and claudin 5 (CLDN5) (Fig. 11D) genes. SHDS-treated LSNPs increased only TJP1 and CLDN5, SHDS-treated FNPs increased TJP1, OCLN and CLDN5, SHDS-treated HNPs increased the expression of all these genes, although to a different extent. Interestingly, CNPs were the only NBM that increased the expression of all TJs-encoding genes evaluated both in the untreated (except for CLDN5) and in the SHDS-treated form (Fig. 11).
This up-regulation of TJs genes may suggest a compensatory response mounted by GI cells in response to potentially cytotoxic NBMs. According to the functional results in terms of permeability (Fig. 10B), such response was successful in preventing the loss of barrier integrity.
Finally, we analysed the gene expression of TNF-α and IL-6, two pro-inflammatory cytokines involved in the pathogenesis of inflammatory bowel disease , opposed to IL-10, known for its immune-suppressive role in inflammatory bowel disease , and to IL-22, which triggers regeneration after intestinal injuries  and preserves the intestinal epithelial integrity .
None of the untreated NBMs significantly increased the cytokines gene expression (Fig. 12), in line with the low modulation of TJ-genes (Fig. 11). SHDS-treated CNPs did not increase the expression of pro-inflammatory TNF, which was instead increased by SHDS-treated LSNPs, FNPs and HNPs (Fig. 12A). All the SHDS-treated NBMs increased IL6 (Fig. 12B), but they also up-regulated the anti-inflammatory/immune-suppressive cytokines IL10 (Fig. 12C) and IL22 (Fig. 12D), suggesting a balance between pro-inflammatory and anti-inflammatory processes that could contribute to preserve the GI barrier integrity.
NBM intestinal barrier crossing
The results obtained with the Lucifer Yellow test suggested that the tested NBMs are unable to cross the barrier, even after SHDS-treatment. To monitor the NBM possible transcellular translocation, the barrier model was exposed to CNPs and FNPs and the particle concentration in the basolateral compartment of Caco-2 GI barrier was monitored by Nanoparticle Track Analysis (NTA). These samples were selected because the technique is more sensible on samples with a highly refractive index. No particles were found in the basolateral compartment after treatment with both SHDS-treated and untreated CNPs and FNPs (data not shown). These data were confirmed for FNPs using the FerroZine™ assay which showed no significant presence of iron (data not shown).
The exposure to NBMs is becoming more and more common due to their widespread use in various industrial sectors including food and medicine. Consequently, the number of studies focusing on NBMs hazard are increasing exponentially [73,74,75]. Ingestion has been recognized as an important route of exposure to both nanomaterials and NBMs only recently. For this reason it has been little investigated so far. Moreover, because of the complexity of the OGI tract physiology, a consensus on the most suitable models and markers for the assessment of NBM toxicity has not been reached yet.
Recently, several cellular models have been proposed to mimic the manifold gut anatomy and physiology [32, 33, 76,77,78,79]. However, in most of the existing studies cells are exposed to untreated NBMs, neglecting the transformations that occur to NBMs during the transit in the OGI tract . Recently, different in vitro systems simulating digestion have been proposed to monitor such biotransformation [50, 80, 81]. Nevertheless, few studies have been published on the impact that the NBM biotransformation along the OGI tract may have on their toxicity toward intestinal cells [39, 52,53,54, 82].
In the present study we found that the application of an in vitro Simulated Human Digestion System (SHDS) induces a significant modification of the bioidentity of four NBMs, which in turn modulates their bioactivity towards intestinal epithelial cells. Samples representative of NBMs with potential applications in oral drug delivery (FNPs, CNPs, HNPs, LSNPs) [55,56,57,58] or as ingredients of nutraceutical formulations have been selected (LSNPs) .
NBMs acquire a new identity in the OGI tract
The concept that the NBM bioactivity strongly depends upon their physical and chemical properties is currently well consolidated. Size and surface properties are the parameters which have been recognized to modulate the NBM toxicity [84,85,86].
Size primarily affects dosimetry and cellular uptake. Smaller particles can penetrate cells more easily by active processes such as caveolae- and clathrin-mediated endocytosis, or by passive diffusion across the cell membrane . On the other hand, size affects particle sedimentation and diffusion, thus modifying the kinetics of contact with cells and the effective dose [88, 89].
An increase of the particles size consequent to aggregation or agglomeration following contact with simulated gastric or intestinal fluids has been previously reported for several types of NBMs, as lipid nanoparticles , Ag nanoparticles [52, 91, 92], TiO2 nanoparticles [39, 93], silica nanoparticles [52, 94], amorphous Mg-Ca phosphate nanoparticles , Au nanoparticles , and others [97, 98]. Our study confirms previous reports, since a significant increase of the size has been observed for all the NBMs investigated (Fig. 2). More importantly, we demonstrate that this process, occurring mainly in the gastric compartment, is irreversible regardless of the chemical composition of the NBMs. In fact, all NBMs appear aggregated in the cell media, and in these forms have a higher probability to interact with the intestinal cells in vivo. The low pH and the high ionic strength of the gastric fluid are the main driving force of aggregation, as demonstrated for stabilized zero-valent iron nanoparticles  and Au nanoparticles , while proteins in the medium appear to partially inhibit the process.
However, aggregation is not the only transformation process that NBMs undergo. In fact, in the case of HNPs, LSNPs and FNPs the aggregates appear composed of particles smaller than the untreated ones. Dissolution, enzymatic degradation or coating degradation were observed, in line with other studies reporting that extreme pH can dissolve pH-sensitive NBMs , and that enzymes and proteins can contribute to NBMs dissolution by digesting NBMs components .
Another important aspect is the modification of the NBMs surface chemistry. Surface charge both affects colloidal stability and nanoparticles-membrane interaction [103,104,105]. On the other hand, the NBM surface acts as a scaffold that binds proteins and biomolecules, leading to the acquisition of a new biological identity [106,107,108,109,110] that influences the NBMs affinity for different cell types and specific receptors [51, 87]. The composition of bio-molecular corona and subsequent NBMs activity strongly depend on the specific bio-fluid in which they are dispersed [111,112,113,114].
Our study clearly shows that proteins and other components (e.g., bile salts) can irreversibly bind to the surface by forming a hard corona. Clear-cut differences in the bio-molecular corona were found between untreated FNPs and SHDS-treated FNPs. Indeed, SDS-PAGE and mass spectrometry identified different proteases derived from SHDS. This corona also partially protects HNPs and LSNPs from degradation. The protective effect of proteins has been previously observed for hydroxyapatite nanoparticles after the addition of milk to the in vitro digestive process, resulting in a delayed dissolution due to the proteins coating . Moreover, Levak et al., and Martin et al. demonstrate a minor release of Ag+ ions by silver nanoparticles when coated with proteins [116, 117]. On the other hand, the bio-molecular corona modifies the surface charge, but does not completely inhibit the surface reactivity of CNPs and FNPs, suggesting that the surface of the particles is still partially exposed to the solvent, and can interact directly with the cells. This effect is clearly dependent on the nature of the materials. Indeed, we have previously reported that in the case of TiO2 the treatment with the SHDS completely inhibited the surface reactivity . These results underline the importance of the presence of active components in SHDS to accurately describe the NBMs transformation.
Effect of the biotransformation on the toxicity of NBMs toward intestinal cells
The pre-treatment with the SHDS largely affected the behaviour of NBMs toward Caco-2 cells. However, the effects were different, depending on the type of NBMs and on the model/endpoint. The treatment increased the toxicity of LSNPs toward undifferentiated Caco-2 cells, likely because of the degradation of the outermost layers’ and the release of the surfactants, induced by the SHDS. On the contrary, the SHDS did not change the cytotoxicity of CNPs, and reduced the cytotoxicity of FNPs and HNPs (Fig. 8). The trend was different in primary epithelial intestinal cells. In this case, SHDS increased the toxicity of CNPs and FNPs, while LSNPs and HNPs maintained a toxicity trend like those observed in Caco-2 cells (Fig. 9). Overall, the primary cells appeared to be more sensitive to homeostatic perturbations. This finding is in line with other non-transformed cell lines as CCD-841, which showed a stronger decrease in viability after treatment with isothiocyanate-capped silicon nanoparticles in comparison with Caco-2 cells . Our results suggest that the use of primary epithelial cells helps in obtaining a more complete picture of the effects of NBMs in humans, integrating the results obtained on immortalized cells, useful for preliminary and large-scale screenings, with the results obtained in a model closer to the cells of the human GI tract. However, we recommend to use both these models in parallel, in order to obtain multiple information at the same time: if on the one hand, primary cells gives more reliable information on the toxicity outcome in non-transformed gastro-intestinal tissue, on the other hand the use of immortalised cells that can form a competent gastrointestinal barrier allows to obtain information about the impact of NBMs on the barrier integrity.
Interestingly, both treated and untreated NBMs were not cytotoxic in the differentiated Caco-2 cells and did not alter the permeability of the intestinal barrier, while a clear perturbation of the TJs was observed for all NBMs. This may be interpreted as a compensatory mechanism: to limit the damage induced by NBMs, GI cells likely respond by increasing the expression of specific genes encoding for the main TJs proteins. By increasing the amount of TJs complexes, this response maintains the GI barrier intact, as it occurs as a compensatory mechanism in different diseases  or in response to IL-10, a cytokine increased by NBMs in our model and known to preserve the GI barrier integrity . Indeed, while the pro-inflammatory cytokines TNF-α and IL-6, whose genes also are up-regulated by NBMs, are known to promote the disruption of the GI barrier , also IL-10 is concurrently over-expressed after the exposure to NMBs: this balance may promote the recovery of the barrier integrity after an initial inflammation-related damage. The induction of TJ protein genes was much more evident in SHDS-treated samples. This might be due to the presence of proteases derived from the SHDS in the hard corona, as demonstrated for FNPs. In fact, protease/antiprotease balance has been reported to be important in maintaining and regulating the intestinal permeability . On the other hand, this effect could be compensated by the high presence of protease inhibitors derived from the cell media. This hypothesis should not necessarily apply to the other NBMs tested, since the protein corona composition is dependent on the chemical nature of the NBM. Conversely, it has been reported that TiO2 nanoparticles down-regulated TJs in vivo and ex vivo in mice, increasing paracellular permeability . In some cases, it is the combination of NBMs as TiO2 or SiO2 with additives found in food  or with bacterial toxins as lipopolysaccharide  to reduce TJ, adherens junction and gap junction proteins . Since no increase in the permeability of Lucifer Yellow was detected in our experimental conditions for all the NBMs tested, we concluded that the increase in TJs genes elicited by NBMs was sufficient to prevent any loss of GI barrier integrity. Alternatively, we cannot exclude that the integrity of the GI barrier that we measured was the result of a complete process of barrier reparation after an initial damage: indeed, it has been documented that Caco-2 cells exposed to silica nanoparticles undergo to an initial disruption of actin cytoskeleton and TJs architecture, followed by a recovery phase of actin remodelling and TJs reassembly . We recognize that one limitation of our work is that we studied the acute effects only. Indeed, our main focus was the acute toxicity of NBMs, because the NBMs studied are used for medical purposes. Therefore, the exposure to the gastrointestinal cells is acute and not chronic. As follow up, we plan to monitor the TJ changes over time, in order to have a deeper insight into the time-dependent modulation of these parameters, focusing on NBMs whose exposure is chronic for environmental or occupational reasons.
As expected, both untreated and treated FNPs and CNPs did not cross the barrier by transcellular or paracellular routes.
Since NBMs are not-self components it has been widely reported that the exposure of GI barrier to NBMs induces local inflammation, supported by the presence of abundant lymphoid tissues associated with the intestinal mucosa  and/or by alterations in the gut microbiota . Also, epithelial cells physiologically produce cytokines and chemokines that are critical in controlling the immune cells activation and the homeostasis of microbiota . An altered production of cytokines from epithelial cells may result in dysbiosis, pathogenic infections or inflammatory bowel disease . As final parameter of biocompatibility, we thus evaluated how the NBMs tested may alter the production of pro-inflammatory and anti-inflammatory cytokines by Caco-2 cells. The increase expression in typical pro-inflammatory cytokines as TNF and IL6, but also in anti-inflammatory cytokines as IL10 and in IL22, related to GI epithelial regeneration, elicited by NBMs may suggest the development of inflammatory events induced by NBMs exposure, paralleled by a compensatory secretion of anti-inflammatory and pro-regenerative cytokines. This balance, together with the over-expression of TJ genes, likely contributes to prevent barrier damage and integrity loss. Our data are in line with the work of Colombo and co-workers, reporting that commercial ZnO nanoparticles increase IL-6 and IL-8 production in Caco-2 barrier model, maintaining barrier integrity . Similarly, polyvinyl chloride particles have been reported to induce IL-1β secretion without altering Caco-2/HT29-MTX/THP1 barrier integrity and viability . All these works, however, do not consider the transformation that occurs during the NBM digestion. Indeed, in the case of SHDS-treated NBMs, we observed a significantly stronger increase of TJ and cytokine genes, likely because of the dramatic modifications experienced by the NBMs following the treatment with the SHDS. However, the lack of increased permeability in Caco-2 barrier exposed to SHDS-treated NBMs indicates that these modifications are coupled with preserved barrier integrity. Notably, CNPs had the lower effects on TJs and cytokines genes even after digestion, confirming themselves as the NBMs less modified during GI transit and more biocompatible after oral ingestion.
In this work we developed a robust and consolidated pipeline that combines deep chemical-physical characterization techniques, microscopic analysis, simulated digestion and read-out of biological events, including biological assays on primary cells, to provide information on the toxicity in non-transformed gastro-intestinal tissue, and on barrier-forming immortalized cells, to obtain information about gastrointestinal barrier integrity and inflammatory events, after acute exposure to NBMs. Overall, the results add a piece of evidence on the importance of associating validated chemical and microscopic characterization, SHDS methods and in vitro models for the assessment of NBM intestinal acute toxicity and biocompatibility. Our pipeline is versatile, meaning that it can be applied to different NBMs that can be ingested accidentally, for environmental or occupational reasons. At the same time, it could provide a huge amount of information on NBMs transformation and acute effects on gastrointestinal tract cells. Further studies will be necessary to validate the reported results in vivo.
Materials and methods
Materials and reagents
Plasticware for cell cultures was from Falcon (Becton Dickinson, Franklin Lakes, NJ). FBS and culture medium were from Invitrogen Life Technologies (Carlsbad, CA). If not otherwise specified, reagents were purchased from Sigma-Merck.
CNPs were synthesized by hydrothermal carbonization of glucose, following a protocol previously described . CNPs are composed of elemental carbon, mainly amorphous, and are produced as colloidal suspension in water.
LSNPs, developed by Nanovector srl, Torino, Italy, are composed by water (Citrate/Phosphate buffer pH 5), glycerol, soy lecithin, glyceryl citrate/lactate/oleate/linoleate (E-472), glycerol monostearate (E-471), polysorbate 20, ascorbyl palmitate, sodium benzoate, α-tocopheryl acetate, strawberry flavour, sucralose and loaded with Melatonin (0.1% (w/w)). FNPs are a colloidal suspension in phosphate buffer (1 mM) of Fe3O4 nanoparticles embedded in a polymeric matrix (poly-lactic-co-glycolic acid/polyethylene glycol) developed by Colorobbia Consulting, Vinci, Italy.
HNPs have been purchased by Sigma Aldrich (Merck KGaA, Darmstadt, Germany) in the form of a powder made of pure hydroxyapatite with stoichiometric composition (Ca5(PO4)3OH).
Dynamic light scattering (DLS)
Size distribution and polydispersity index (PDI) were measured on SHDS-treated and untreated NBMs diluted in ultrapure water (100 µg/ml) or in cell medium (DMEM supplemented with 10% FBS, 1% penicillin/streptomycin solution) (100 µg/ml). Measurements were performed by using the Zetasizer, Nano instrument (Malvern Instruments, Malvern, UK) with a 633 nm HeNe laser. Instrument settings were: replicate 3, equilibrium time 60 s, T = 25 °C, dispersant refractive index 1.330 (water) and 1.345 (cell medium), dispersant viscosity 0.8872 cP (water) and 0.8000 cP (cell medium), material refractive index 1.410 (LSNPs), 2.420 (CNPs), 2.420 (FNPs) and 1.650 (HNPs), material absorption 1.000.
Untreated CNPs, LSNPs and FNPs were diluted in ultrapure water before the analysis, while HNPs were suspended in ultrapure water and sonicated for 5 min with a probe sonicator (Sonoplus HD3100 Bandelin, Microtip MS73, diameter 3 mm, power 100 W, amplitude 30%). SHDS-treated NBMs were analysed in the fluids without dilution. In each experiment three subsequent measurements were performed on the same suspension. The data were expressed as the mean of three independent experiments, ± standard deviation. Each line represents the mean values of 15 measurements that were obtained in three independent experiments.
Electrophoretic light scattering (ELS)
ζ-potential was measured using an electrophoretic light scattering analyzer (Zetasizer, Nano ZS Malvern Instruments, Malvern, UK). For ζ-potential curve versus pH, NBMs were diluted at 500 µg/ml in ultrapure water and pH was modified by adding NaOH 0.1 M or HCl 0.1 M. Instrument settings were: dispersant (water) dielectric constant: 78.5.
Flow particle imaging analysis (FPIA)
FPIA was performed by using a Sysmex FPIA3000 analyser. High power field (2 × secondary lens) was applied, which allows measuring particles from 1 to 40 μm. The suspensions of nanoparticles in simulated digestive fluids were centrifuged at 8000 rpm for 10 min by Rotina 380 R (Hettich Zentrifuger). The suspensions were pelleted, the supernatant was removed, and the resulting pellets were resuspended in ultrapure water for 2 min in an ultrasonic bath. The washing process was repeated three times and 5 ml of the suspensions were analysed.
The NBM surface reactivity was monitored by EPR analysis (Miniscope 100 EPR spectrometer, Magnettech, Berlin, Germany) using TEMPONE-H (1-hydroxy-2,2,6,6-tetramethyl-4-oxo-piperidine, Enzo Life Sciences, Inc.) as spin probe. Suspension of untreated or SHDS-treated NBMs in ultrapure water or cell medium (0.5 mg/ml) was diluted 1:1 in a 100 µM solution of Tempone-H and the suspension constantly stirred in a glass vial. The EPR spectra were recorded on a sample aliquot (50 µl). Instrument settings: microwave power 7 mW, modulation amplitude 1 G, scan time 80 s, two scans.
Transmission electron microscope (TEM) measurements
TEM was accomplished utilizing a FEI CM20 microscope operating at 200 kV. TEM samples were prepared by placing one drop of a diluted sample on a carbon-coated Cu grid and allowing the solvent to evaporate.
Protein corona analysis
NBMs were treated with SHDS following the protocol explained below. Treated and untreated NBMs were incubated for 24 h in DMEM 10% FBS, 1% penicillin/streptomycin at 37 °C under agitation (0.5 mg/ml). After the incubation, the NBM-corona complex was isolated through three centrifugation/dispersion cycles in PBS. For FNPs, ferromagnetic spheres were used to isolate the complex NBMs-corona (unpublished data). For SDS-PAGE, the pellets obtained after the washing were stripped using a loading buffer (Cell Signalling Technology) in 0.1 M dithiothreitol and heated at 100 °C. The obtained solutions were centrifuged before loading the samples in a 10% acrylamide gel. SDS-PAGE was carried out using the Mini-Protean (BioRad) system at 120 V until the dye front reached the end of the gel. The gels were stained using Coomassie (Thermo Scientific) and scanned with the Amersham Gel doc system.
For the mass spectrometry analysis, the samples in-gel were digested with trypsin and treated with different solutions to extract the peptides from the gel matrix. Raw mass spectrometry data were processed using the MaxQuant version 184.108.40.206. . The identification of peptides and proteins was done using the UniProt database. Perseus software version 220.127.116.11  allowed the analysis of the LFQ intensities obtained. Data were log transformed and missing values were replaced with values from a normal distribution.
Caco-2 epithelial colon cells were obtained from American Tissue Culture Collection (ATCC) and were grown in DMEM supplemented with 20% FBS, 1% penicillin/streptomycin. For the experiments, cells were used between passage 33 and 47, and incubated in DMEM supplemented with 10% FBS, 1% penicillin/streptomycin. To obtain Caco-2 monolayer forming a competent intestinal barrier model, cells were grown on Millicell®-96 cell culture inserts (Merck KGaA, Darmstadt, Germany) for 21 days .
HCT116 cells were obtained from the European Collection of Authenticated Cell Cultures (ECACC, catalogue No. #91,091,005) and were grown and exposed to NBMs in McCoy's 5a medium containing 2 mM glutamine, 10% FBS and 1% penicillin/streptomycin. Cells were used between passage 15 and 25.
Human colonic epithelial cells (HCoEpiC) were purchased from CliniSciences (CliniSciences, Guidonia Montecelio, Italy) and were cultured in Colonic Epithelial Cell Medium (HCoEpiCM) supplemented with 10% (v/v) Colonic Epithelial Cell Growth Supplement (HCoEpiCGS) and 1% penicillin/streptomycin. Experiments were performed between the passage 5 and 8.
Preparation of simulated digestive fluids
Simulated digestive fluids were prepared following the protocol used by Sohal et al. . The composition of each simulated digestive fluid is summarized in Table 4. For each fluid, the organic and inorganic parts were prepared separately by adding the components to ultrapure water and dissolving them under magnetic stirring. Then, the two solutions were mixed in a ratio of 1:1 (v/v) and stirred overnight.
The active components were added just before performing the experiment and the solution was vortexed to suspend them.
Simulated human digestion system
The protocol used for the simulated human digestion system (SHDS) is that used by Sohal et al. .
A NBM suspension at the concentration of 1 mg/ml was SHDS-treated using an equal volume of simulated digestive fluids (Additional file 1: Fig S10). First, the SSF was added and the sample was incubated for 15 min at 37 °C under shaking. After this time, SGF was added and incubated for 4 h. Finally, SIF, composed of simulated duodenal fluid (SDF) and simulated bile fluid (SBF) in a ratio of 2:1 (v/v), was added and incubated for further 4 h. The ratio of simulated digestive fluids was 1:2:3 (Additional file 1: Fig S10). Table 4 summarises the simulated digestive fluids composition. At the end of the process, if necessary, pH was adjusted in the range of 6.5 and 7.5 using 1 M NaHCO3 and the suspension was sterilized 15 min under UV radiations.
For surface reactivity evaluation the suspension was centrifuged at 11,000 rpm (Rotina 380 R, Hettich Zentrifuger) and, after discarding the supernatant, it was resuspended in cell culture medium in a volume depending on the desired concentration.
For other tests the suspension was mixed with cell medium to obtain the final concentration. Incubation with cells or intestinal barrier model was performed for 24 h.
WST-1 assay, based on the cleavage of the slightly red tetrazolium salt WST-1 (4-[3-(4-iodophenyl)-2-(4-nitrophenyl)-2H-5-tetrazolio]-1,3-benzene disulfonate) to form a dark red formazan dye by metabolically active cells, was used to evaluate the cell viability, as index of mitochondrial activity, after the treatment with NBMs. WST-1 was added at 10% (v/v) of cell medium and the absorbance was read at 440 nm after 2 h for Caco-2 cells, 1 h and 30 min for HCT116 cells, 4 h for HCoEpiC cells and 30 min for the intestinal barrier model using a Synergy HT Multi-Detection Microplate Reader (Bio-Tek Instruments, Winooski, VT) or a Spectramax ID3 plate reader (Molecular Devices, for HCT116 cells only). The absorbance value at the reference wavelength (630 nm) was subtracted.
Genotoxicity was assessed by counting the DNA double strand break repair foci, after immunostaining of the 53BP1 DNA repair protein, as previously described [21, 133]. Briefly, after exposure to NBMs, cells were fixed with 4% paraformaldehyde, and permeabilized with 0.2% v/v Triton X-100 prepared in PBS containing 3% w/v bovine serum albumin (PBS-BSA). Non-specific sites were blocked with PBS-BSA, then incubated for 1 h with rabbit polyclonal anti-TP53BP1 antibody (Abnova, reference PAB12506) diluted in PBS-BSA, washed three times for 5 min with PBS-BSA and incubated for 1 h with an anti-rabbit IgG Atto 633 antibody (Sigma-Aldrich, 41,176) diluted in PBS-BSA. After three washing in PBS-BSA containing 0.2% Triton X-100, the nuclei were stained with 0.3 μg/ml Hoechst 33,342 (Sigma-Aldrich) for 20 min at room temperature. The number of cell nuclei and the average number of 53BP1 foci per cell nucleus were counted using a CellInsight CX5 High-Content Screening Platform (Thermo Fisher Scientific). This experiment was repeated three times independently, with n = 5 replicates in each independent experiment.
Trans-Epithelial Electrical Resistance (TEER)
To evaluate the barrier formation and integrity of Caco-2 barrier model after the exposure to NBMs, TEER was measured using the Millicell® ERS-2 voltohmmeter (Merck KGaA, Darmstadt, Germany). The resistance was read in ohms and the resistivity was calculated by subtracting the cell-free inserts value from the cell-containing inserts, multiplying for the cells growth area. Only the monolayer with values > 250 Ω*cm2 were used for exposure to NBMs.
Evaluation of barrier permeability
To evaluate the permeability of the intestinal barrier model the trans-epithelial passage of Lucifer Yellow fluorescent dye  was measured following the NANoREG SOP (Standard Operating Procedure for evaluation of NPs impact on Caco2 cell barrier model). After collection of the medium, the cells and the basolateral compartment of Millicell®-96 cell culture inserts were rinsed thrice with Hanks’ Balanced Salt Solution (HBSS). Then 50 µl/well of a 0.4 mg/ml Lucifer Yellow solution in HBSS were added in the apical compartment. After 2 h of incubation at 37 °C, the apparent permeability (Papp) and the percentage of fluorophore recovered from the lower chamber in cell-free inserts were calculated, reading the relative fluorescence units (RFUs) (λ excitation: 504 nm, λ emission: 529 nm), with a Synergy HT Multi-Detection Microplate Reader.
NBMs absorption through the intestinal barrier by Nanoparticle Tracking Analysis (NTA)
The CNPs and FNPs passage through the Caco-2 intestinal barrier was evaluated by measuring the number of particles in the initial suspension and in the basolateral compartment of the Millicell®-96 cell culture inserts using Nanoparticle Tracking Analysis (NTA, ZetaView, Particle Metrix GmbH, Germany). The samples were diluted in ultrapure water before the analysis. Sensitivity was set at 60 and shutter value at 100. In this condition neither phenol red nor FBS interference was detected.
FNPs absorption through the intestinal barrier by colorimetric assay
For the quantification of FNPs in the basolateral compartment the FerroZine™-based colorimetric assay was used based on the protocols reported by Balivada and co-workers  and by Jeinter . First, to dissolve and reduce the iron contained in FNPs, 150 µl of the samples were incubated at 70 °C for 2 h with 150 µl of 1.2 M HCl and 60 µl of 1 M ascorbic acid. Then, 300 µl of the resulting solution were incubated with 200 µl of 1.5 M sodium acetate, 50 µl of 1 M ascorbic acid, 350 µl of ultrapure water, and 100 µl of 21 mM FerroZine™ (Thermo Fisher Scientific). After 20 min of incubation at room temperature, the absorbance at 562 nm was measured by an UV–Vis spectrophotometer (UVICON 930, Kontron Instruments, Basel, Switzerland) and the concentration was calculated using a calibration curve.
Quantitative Real-Time PCR (qRT-PCR)
mRNA was extracted using the phenol/chloroform/ethanol method: cells were lysed in 0.5 ml RiboZol (VWR; Radnor, PA) and incubated for 10 min at room temperature, and then 0.2 ml chloroform was added. Samples were shaken for 15 s and incubated at room temperature for 3 min before being centrifuged for 15 min at 12,000g at 4 °C. Aqueous phase was transferred in a new tube and 0.2 ml isopropanol was added, the samples were incubated for 10 min at room temperature before centrifugation at 12,000g for 10 min at 4 °C. RNA pellets were washed twice with ethanol 70% v/v by centrifuging at 12,000g for 5 min at 4 °C, and were resuspended in RNAse-free water. The RNA quantification was performed using the Take3 plate (Synergy HT Multi-Detection Microplate Reader), reading the absorbance at 260 nm. The reverse transcription of RNA samples was performed using the iScript cDNA synthesis kit (Bio-Rad, Segrate, Italy), according to the manufacturer’s instructions.
To quantify the expression of CLDN3, CLDN5, OCLN, TJP1, IL-6, IL-10, IL-22 and TNF-α, qRT-PCR was carried out using as gene reference the ribosomal protein unit S14 coding gene. Briefly, 5 µl of iTaq Universal SYBR Green Supermix (Bio-Rad Laboratories), 2 µl of 5 µM primers mix (Table 5) and 3 µl of cDNA (5 ng/µl) were used for each sample. Samples were run using a CFX96 Real-Time System (Bio-Rad Laboratories) for 30 s at 95 °C, 5 s at 95 °C and 30 s at 60 °C for 42 cycles. The analysis was performed using Bio-Rad CFX Maestro software (Bio-Rad Laboratories).
Statistics were performed using ANOVA (ANalysis Of VAriance) with post-hoc Tukey Honestly Significant Difference Test Calculator for comparing multiple treatments , using Statistical Package for Social Science software (IBM SPSS Statistics v.19). p < 0.05 was considered significant.
Availability of data and materials
All data generated or analysed during this study are included in this published article and its additional files.
Tumour Suppressor P53-binding Protein 1
ANalysis Of VAriance
Bovine serum albumin
Claudin encoding gene
- dH :
Dynamic light scattering
Dulbecco's modified eagle medium
Electrophoretic light scattering
Electron paramagnetic resonance spectroscopy
Foetal bovine serum
Flow particle imaging analysis
Hanks’ Balanced Salt Solution
Label free quantification
Lipid surfactant nanoparticles
Nanoparticle tracking analysis
Occludin encoding gene
Phosphate buffered saline
Quantitative Real Time-Polymerase Chain Reaction
Relative fluorescence units
Simulated bile fluid
Simulated duodenal fluid
Sodium Dodecyl Sulphate-PolyAcrylamide Gel Electrophoresis
Standard error of the mean
Simulated gastric fluid
Simulated human digestion system
Simulated intestinal fluid
Simulated saliva fluid
Transmission electron microscope
Tumour necrosis factor
Zonula Occludens encoding gene
Conte A, Longano D, Costa C, Ditaranto N, Ancona A, Cioffi N, et al. A novel preservation technique applied to fiordilatte cheese. Innov Food Sci Emerg Technol. 2013;19:158–65.
da Costa BS, Bresolin JD, Sivieri K, Ferreira MD. Low-density polyethylene films incorporated with silver nanoparticles to promote antimicrobial efficiency in food packaging. Food Sci Technol Int. 2020;26:353–66.
Esfahani R, Jafari SM, Jafarpour A, Dehnad D. Loading of fish oil into nanocarriers prepared through gelatin-gum Arabic complexation. Food Hydrocoll. 2019;90:291–8.
Pulit-Prociak J, Chwastowski J, Siudek M, Banach M. Incorporation of metallic nanoparticles into cosmetic preparations and assessment of their physicochemical and utility properties. J Surfactants Deterg. 2018;21:575–91.
Jiménez-Pérez ZE, Singh P, Kim YJ, Mathiyalagan R, Kim DH, Lee MH, et al. Applications of Panax ginseng leaves-mediated gold nanoparticles in cosmetics relation to antioxidant, moisture retention, and whitening effect on B16BL6 cells. J Ginseng Res. 2018;42:327–33.
Yang X, Yang F, Walboomers XF, Bian Z, Fan M, Jansen JA. The performance of dental pulp stem cells on nanofibrous PCL/gelatin/nHA scaffolds. J Biomed Mater Res Part A. 2010;93A:247–57.
Adamiak M, Cheng G, Bobis-Wozowicz S, Zhao L, Kedracka-Krok S, Samanta A, et al. Induced pluripotent stem cell (iPSC)-derived extracellular vesicles are safer and more effective for cardiac repair than iPSCs. Circ Res. 2018;122:296–309.
González-Fernández Y, Zalacain M, Imbuluzqueta E, Sierrasesumaga L, Patiño-García A, Blanco-Prieto MJ. Lipid nanoparticles enhance the efficacy of chemotherapy in primary and metastatic human osteosarcoma cells. J Drug Deliv Sci Technol. 2015;30:435–42.
González-Fernández Y, Imbuluzqueta E, Zalacain M, Mollinedo F, Patiño-García A, Blanco-Prieto MJ. Doxorubicin and edelfosine lipid nanoparticles are effective acting synergistically against drug-resistant osteosarcoma cancer cells. Cancer Lett. 2017;388:262–8.
do Pereira AES, Oliveira HC, Fraceto LF. Polymeric nanoparticles as an alternative for application of gibberellic acid in sustainable agriculture: a field study. Sci Rep. 2019;9:7135.
Pandey K, Anas M, Hicks VK, Green MJ, Khodakovskaya MV. Improvement of commercially valuable traits of industrial crops by application of carbon-based nanomaterials. Sci Rep. 2019;9:19358.
Pietroiusti A, Bergamaschi E, Campagna M, Campagnolo L, De Palma G, Iavicoli S, et al. The unrecognized occupational relevance of the interaction between engineered nanomaterials and the gastro-intestinal tract: a consensus paper from a multidisciplinary working group. Part Fibre Toxicol. 2017;14:47.
Bouwmeester H, van der Zande M, Jepson MA. Effects of food-borne nanomaterials on gastrointestinal tissues and microbiota. WIREs Nanomed Nanobiotechnol. 2018;10:e1481.
Vermette D, Hu P, Canarie MF, Funaro M, Glover J, Pierce RW. Tight junction structure, function, and assessment in the critically ill: a systematic review. Intensive Care Med Exp. 2018;6:37.
Oshima T, Miwa H, Joh T. Changes in the expression of claudins in active ulcerative colitis. J Gastroenterol Hepatol. 2008;23:S146–50.
Zeissig S, Bürgel N, Günzel D, Richter J, Mankertz J, Wahnschaffe U, et al. Changes in expression and distribution of claudin 2, 5 and 8 lead to discontinuous tight junctions and barrier dysfunction in active Crohn’s disease. Gut. 2007;56:61–72.
Cornu R, Chrétien C, Pellequer Y, Martin H, Béduneau A. Small silica nanoparticles transiently modulate the intestinal permeability by actin cytoskeleton disruption in both Caco-2 and Caco-2/HT29-MTX models. Arch Toxicol. 2020;94:1191–202.
Ruiz PA, Morón B, Becker HM, Lang S, Atrott K, Spalinger MR, et al. Titanium dioxide nanoparticles exacerbate DSS-induced colitis: role of the NLRP3 inflammasome. Gut. 2017;66:1216–24.
Sohal IS, O’Fallon KS, Gaines P, Demokritou P, Bello D. Ingested engineered nanomaterials: state of science in nanotoxicity testing and future research needs. Part Fibre Toxicol. 2018;15:29.
Farcal L, Torres Andón F, Di Cristo L, Rotoli BM, Bussolati O, Bergamaschi E, et al. Comprehensive in vitro toxicity testing of a panel of representative oxide nanomaterials: first steps towards an intelligent testing strategy. PLoS ONE. 2015;10:e0127174.
Dorier M, Tisseyre C, Dussert F, Béal D, Arnal ME, Douki T, et al. Toxicological impact of acute exposure to E171 food additive and TiO2 nanoparticles on a co-culture of Caco-2 and HT29-MTX intestinal cells. Mutat Res Toxicol Environ Mutagen. 2019;845:402980.
Dorier M, Béal D, Tisseyre C, Marie-Desvergne C, Dubosson M, Barreau F, et al. The food additive E171 and titanium dioxide nanoparticles indirectly alter the homeostasis of human intestinal epithelial cells in vitro. Environ Sci Nano. 2019;6:1549–61.
Dorier M, Béal D, Marie-Desvergne C, Dubosson M, Barreau F, Houdeau E, et al. Continuous in vitro exposure of intestinal epithelial cells to E171 food additive causes oxidative stress, inducing oxidation of DNA bases but no endoplasmic reticulum stress. Nanotoxicology. 2017;11:751–61.
Basak SC, Vracko M, Witzmann FA. Mathematical nanotoxicoproteomics: quantitative characterization of effects of multi-walled carbon nanotubes (MWCNT) and TiO2 Nanobelts (TiO2-NB) on protein expression patterns in human intestinal cells. Curr Comput Aided Drug Des. 2016;12:259–64.
Lai X, Agarwal M, Lvov YM, Pachpande C, Varahramyan K, Witzmann FA. Proteomic profiling of halloysite clay nanotube exposure in intestinal cell co-culture. J Appl Toxicol. 2013;33:1316–29.
Lai YH, D’Souza MJ. Microparticle transport in the human intestinal M cell model. J Drug Target. 2008;16:36–42.
Stagg AJ. Intestinal dendritic cells in health and gut inflammation. Front Immunol. 2018;9:2883.
Yang R, Liao Y, Wang L, He P, Hu Y, Yuan D, et al. Exosomes derived from M2b macrophages attenuate DSS-induced colitis. Front Immunol. 2019;10:2346.
Al-Sadi R, Boivin M, Ma T. Mechanism of cytokine modulation of epithelial tight junction barrier. Front Biosci. 2009;14:2765–78.
Susewind J, de Souza C-W, Repnik U, Collnot E-M, Schneider-Daum N, Griffiths GW, et al. A 3D co-culture of three human cell lines to model the inflamed intestinal mucosa for safety testing of nanomaterials. Nanotoxicology. 2016;10:53–62.
Leonard F, Ali H, Collnot E-M, Crielaard BJ, Lammers T, Storm G, et al. Screening of budesonide nanoformulations for treatment of inflammatory bowel disease in an inflamed 3D cell-culture model. Altex. 2012;29:275–85.
Meirelles GC, Mendes C, Caon T, Teixeira HF, von Poser G, Ponchel G. Intestinal permeability enhancement of benzopyran HP1-loaded nanoemulsions. Eur J Pharm Sci Off J Eur Fed Pharm Sci. 2019;127:115–20.
Krupa L, Bajka B, Staroń R, Dupont D, Singh H, Gutkowski K, et al. Comparing the permeability of human and porcine small intestinal mucus for particle transport studies. Sci Rep. 2020;10:20290.
Tada-Oikawa S, Eguchi M, Yasuda M, Izuoka K, Ikegami A, Vranic S, et al. Functionalized surface-charged SiO(2) nanoparticles induce pro-inflammatory responses, but are not lethal to Caco-2 cells. Chem Res Toxicol. 2020;33:1226–36.
Taboada-López MV, Leal-Martínez BH, Domínguez-González R, Bermejo-Barrera P, Taboada-Antelo P, Moreda-Piñeiro A. Caco-2 in vitro model of human gastrointestinal tract for studying the absorption of titanium dioxide and silver nanoparticles from seafood. Talanta. 2021;233:122494.
Hempt C, Kaiser J-P, Scholder O, Buerki-Thurnherr T, Hofmann H, Rippl A, et al. The impact of synthetic amorphous silica (E 551) on differentiated Caco-2 cells, a model for the human intestinal epithelium. Toxicol In Vitro. 2020;67:104903.
Bertero A, Colombo G, Cortinovis C, Bassi V, Moschini E, Bellitto N, et al. In vitro copper oxide nanoparticle toxicity on intestinal barrier. J Appl Toxicol. 2021;41:291–302.
Vecchiotti G, Colafarina S, Aloisi M, Zarivi O, Di Carlo P, Poma A. Genotoxicity and oxidative stress induction by polystyrene nanoparticles in the colorectal cancer cell line HCT116. PLoS ONE. 2021;16:e0255120.
Marucco A, Prono M, Beal D, Alasonati E, Fisicaro P, Bergamaschi E, et al. Biotransformation of food-grade and nanometric TiO(2) in the oral-gastro-intestinal tract: driving forces and effect on the toxicity toward intestinal epithelial cells. Nanomaterials. 2020;10:2132.
Proquin H, Rodríguez-Ibarra C, Moonen CGJ, Urrutia Ortega IM, Briedé JJ, de Kok TM, et al. Titanium dioxide food additive (E171) induces ROS formation and genotoxicity: contribution of micro and nano-sized fractions. Mutagenesis. 2017;32:139–49.
Jia M, Zhang W, He T, Shu M, Deng J, Wang J, et al. Evaluation of the genotoxic and oxidative damage potential of silver nanoparticles in human NCM460 and HCT116 cells. Int J Mol Sci. 2020;21:1618.
Hayder M, Wojcieszek J, Asztemborska M, Zhou Y, Ruzik L. Analysis of cerium oxide and copper oxide nanoparticles bioaccessibility from radish using SP-ICP-MS. J Sci Food Agric. 2020;100:4950–8.
Shi JH, Axson JL, Bergin IL, Ault AP. Nanoparticle digestion simulator reveals pH-dependent aggregation in the gastrointestinal tract. Anal Chem. 2020;92:12257–64.
Zhou P, Guo M, Cui X. Effect of food on orally-ingested titanium dioxide and zinc oxide nanoparticle behaviors in simulated digestive tract. Chemosphere. 2021;268:128843.
Fadeel B, Feliu N, Vogt C, Abdelmonem AM, Parak WJ. Bridge over troubled waters: understanding the synthetic and biological identities of engineered nanomaterials. WIREs Nanomed Nanobiotechnol. 2013;5:111–29.
Ahmad M, Gani A. Ultrasonicated resveratrol loaded starch nanocapsules: characterization, bioactivity and release behaviour under in-vitro digestion. Carbohydr Polym. 2021;251:117111.
Liang X, Cao K, Li W, Li X, McClements DJ, Hu K. Tannic acid-fortified zein-pectin nanoparticles: stability, properties, antioxidant activity, and in vitro digestion. Food Res Int. 2021;145:110425.
DeLoid GM, Wang Y, Kapronezai K, Lorente LR, Zhang R, Pyrgiotakis G, et al. An integrated methodology for assessing the impact of food matrix and gastrointestinal effects on the biokinetics and cellular toxicity of ingested engineered nanomaterials. Part Fibre Toxicol. 2017;14:40.
Dudefoi W, Rabesona H, Rivard C, Mercier-Bonin M, Humbert B, Terrisse H, et al. In vitro digestion of food grade TiO(2) (E171) and TiO(2) nanoparticles: physicochemical characterization and impact on the activity of digestive enzymes. Food Funct. 2021;12:5975–88.
Sohal IS, Cho YK, O’Fallon KS, Gaines P, Demokritou P, Bello D. Dissolution behavior and biodurability of ingested engineered nanomaterials in the gastrointestinal environment. ACS Nano. 2018;12:8115–28.
Setyawati MI, Zhao Z, Ng KW. Transformation of nanomaterials and its implications in gut nanotoxicology. Small. 2020;16:e2001246.
Llewellyn SV, Kämpfer A, Keller JG, Vilsmeier K, Büttner V, Ag Seleci D, et al. Simulating nanomaterial transformation in cascaded biological compartments to enhance the physiological relevance of in vitro dosing regimes: optional or required? Small. 2021;17:e2004630.
Bitounis D, Parviz D, Cao X, Amadei CA, Vecitis CD, Sunderland EM, et al. Synthesis and physicochemical transformations of size-sorted graphene oxide during simulated digestion and its toxicological assessment against an in vitro model of the human intestinal epithelium. Small. 2020;16:e1907640.
Gerloff K, Pereira DIA, Faria N, Boots AW, Kolling J, Förster I, et al. Influence of simulated gastrointestinal conditions on particle-induced cytotoxicity and interleukin-8 regulation in differentiated and undifferentiated Caco-2 cells. Nanotoxicology. 2013;7:353–66.
Cheng J, Teply BA, Jeong SY, Yim CH, Ho D, Sherifi I, et al. Magnetically responsive polymeric microparticles for oral delivery of protein drugs. Pharm Res. 2006;23:557–64.
Zhao Q, Lin Y, Han N, Li X, Geng H, Wang X, et al. Mesoporous carbon nanomaterials in drug delivery and biomedical application. Drug Deliv. 2017;24:94–107.
Zhang Y, Zhang L, Ban Q, Li J, Li C-H, Guan Y-Q. Preparation and characterization of hydroxyapatite nanoparticles carrying insulin and gallic acid for insulin oral delivery. Nanomedicine. 2018;14:353–64.
Dilnawaz F. Polymeric biomaterial and lipid based nanoparticles for oral drug delivery. Curr Med Chem. 2017;24:2423–38.
Huang Y, Qi M, Zhang M, Liu H, Yang D. Degradation mechanisms of poly (lactic-co-glycolic acid) films in vitro under static and dynamic environment. Trans Nonferr Met Soc China. 2006;16:s293–7.
Schoepf JJ, Bi Y, Kidd J, Herckes P, Hristovski K, Westerhoff P. Detection and dissolution of needle-like hydroxyapatite nanomaterials in infant formula. NanoImpact. 2017;5:22–8.
Feeney OM, Williams HD, Pouton CW, Porter CJH. “Stealth” lipid-based formulations: poly(ethylene glycol)-mediated digestion inhibition improves oral bioavailability of a model poorly water soluble drug. J Control Release. 2014;192:219–27.
Marucco A, Carella E, Fenoglio I. A comparative study on the efficacy of different probes to predict the photo-activity of nano-titanium dioxide toward biomolecules. R Soc Chem. 2015;5:89559–68.
Monopoli MP, Pitek AS, Lynch I, Dawson KA. Formation and characterization of the nanoparticle-protein corona. Methods Mol Biol. 2013;1025:137–55.
Zheng X, Baker H, Hancock WS, Fawaz F, McCaman M, Pungor EJ. Proteomic analysis for the assessment of different lots of fetal bovine serum as a raw material for cell culture. Part IV. Application of proteomics to the manufacture of biological drugs. Biotechnol Prog. 2006;22:1294–300.
Ferruzza S, Rossi C, Scarino ML, Sambuy Y. A protocol for in situ enzyme assays to assess the differentiation of human intestinal Caco-2 cells. Toxicol In Vitro. 2012;26:1247–51.
Peterson MD, Mooseker MS. Characterization of the enterocyte-like brush border cytoskeleton of the C2BBe clones of the human intestinal cell line, Caco-2. J Cell Sci. 1992;102:581–600.
Matsumoto T, Kaifuchi N, Mizuhara Y, Warabi E, Watanabe J. Use of a Caco-2 permeability assay to evaluate the effects of several Kampo medicines on the drug transporter P-glycoprotein. J Nat Med. 2018;72:897–904.
Shekhawat P, Bagul M, Edwankar D, Pokharkar V. Enhanced dissolution/caco-2 permeability, pharmacokinetic and pharmacodynamic performance of re-dispersible eprosartan mesylate nanopowder. Eur J Pharm Sci Off J Eur Fed Pharm Sci. 2019;132:72–85.
Ishiguro Y. Mucosal proinflammatory cytokine production correlates with endoscopic activity of ulcerative colitis. J Gastroenterol. 1999;34:66–74.
Kühn R, Löhler J, Rennick D, Rajewsky K, Müller W. Interleukin-10-deficient mice develop chronic enterocolitis. Cell. 1993;75:263–74.
Lindemans CA, Calafiore M, Mertelsmann AM, O’Connor MH, Dudakov JA, Jenq RR, et al. Interleukin-22 promotes intestinal-stem-cell-mediated epithelial regeneration. Nature. 2015;528:560–4.
Lo BC, Shin SB, Canals Hernaez D, Refaeli I, Yu HB, Goebeler V, et al. IL-22 preserves gut epithelial integrity and promotes disease remission during chronic salmonella infection. J Immunol. 2019;202:956–65.
Miller MR, Raftis JB, Langrish JP, McLean SG, Samutrtai P, Connell SP, et al. Inhaled nanoparticles accumulate at sites of vascular disease. ACS Nano. 2017;11:4542–52.
Milto IV, Ivanova VV, Shevtsova NM, Sukhodolo IV. Rat blood leukocytes after intravenous injection of chitosan-modified magnetic nanospheres. Bull Exp Biol Med. 2020;168:785–8.
Stefaniak AB, Duling MG, Lawrence RB, Thomas TA, LeBouf RF, Wade EE, et al. Dermal exposure potential from textiles that contain silver nanoparticles. Int J Occup Environ Health. 2014;20:220–34.
Lamson NG, Berger A, Fein KC, Whitehead KA. Anionic nanoparticles enable the oral delivery of proteins by enhancing intestinal permeability. Nat Biomed Eng. 2020;4:84–96.
Xavier M, García-Hevia L, Amado IR, Pastrana L, Gonçalves C. In vitro intestinal uptake and permeability of fluorescently-labelled hyaluronic acid nanogels. Int J Nanomed. 2019;14:9077–88.
de Lima IA, Khalil NM, Tominaga TT, Lechanteur A, Sarmento B, Mainardes RM. Mucoadhesive chitosan-coated PLGA nanoparticles for oral delivery of ferulic acid. Artif Cells Nanomed Biotechnol. 2018;46:993–1002.
Tian Y, Xu J, Li Y, Zhao R, Du S, Lv C, et al. MicroRNA-31 reduces inflammatory signaling and promotes regeneration in colon epithelium, and delivery of mimics in microspheres reduces colitis in mice. Gastroenterology. 2019;156:2281-2296.e6.
Lin Q, Liang R, Ye A, Singh H, Zhong F. Effects of calcium on lipid digestion in nanoemulsions stabilized by modified starch: implications for bioaccessibility of β-carotene. Food Hydrocoll. 2017;73:184–93.
Bourlieu C, Ménard O, Bouzerzour K, Mandalari G, Macierzanka A, Mackie AR, et al. Specificity of infant digestive conditions: some clues for developing relevant in vitro models. Crit Rev Food Sci Nutr. 2014;54:1427–57.
Abdelkhaliq A, van der Zande M, Undas AK, Peters RJB, Bouwmeester H. Impact of in vitro digestion on gastrointestinal fate and uptake of silver nanoparticles with different surface modifications. Nanotoxicology. 2020;14:111–26.
Aditya NP, Macedo AS, Doktorovova S, Souto EB, Kim S, Chang P-S, et al. Development and evaluation of lipid nanocarriers for quercetin delivery: a comparative study of solid lipid nanoparticles (SLN), nanostructured lipid carriers (NLC), and lipid nanoemulsions (LNE). LWT Food Sci Technol. 2014;59:115–21.
Nel A, Xia T, Mädler L, Li N. Toxic potential of materials at the nanolevel. Science. 2006;311:622–7.
Fubini B, Ghiazza M, Fenoglio I. Physico-chemical features of engineered nanoparticles relevant to their toxicity. Nanotoxicology. 2010;4:347–63.
Prokopovich P. Interactions between mammalian cells and nano- or micro-sized wear particles: physico-chemical views against biological approaches. Adv Colloid Interface Sci. 2014;213:36–47.
Gehr P. Interaction of nanoparticles with biological systems. Colloids Surf B Biointerfaces. 2018;172:395–9.
Hinderliter PM, Minard KR, Orr G, Chrisler WB, Thrall BD, Pounds JG, et al. ISDD: a computational model of particle sedimentation, diffusion and target cell dosimetry for in vitro toxicity studies. Part Fibre Toxicol. 2010;7:36.
Marucco A, Aldieri E, Leinardi R, Bergamaschi E, Riganti C, Fenoglio I. Applicability and limitations in the characterization of poly-dispersed engineered nanomaterials in cell media by dynamic light scattering (DLS). Mater. 2019;12:3833.
Gonzalez-Paredes A, Torres D, Alonso MJ. Polyarginine nanocapsules: a versatile nanocarrier with potential in transmucosal drug delivery. Int J Pharm. 2017;529:474–85.
Ault AP, Stark DI, Axson JL, Keeney JN, Maynard AD, Bergin IL, et al. Protein corona-induced modification of silver nanoparticle aggregation in simulated gastric fluid. Environ Sci Nano. 2016;3:1510–20.
Walczak AP, Fokkink R, Peters R, Tromp P, Herrera Rivera ZE, Rietjens IMCM, et al. Behaviour of silver nanoparticles and silver ions in an in vitro human gastrointestinal digestion model. Nanotoxicology. 2013;7:1198–210.
Coreas R, Cao X, Deloid GM, Demokritou P, Zhong W. Lipid and protein corona of food-grade TiO(2) nanoparticles in simulated gastrointestinal digestion. NanoImpact. 2020;20:100272.
Sakai-Kato K, Hidaka M, Un K, Kawanishi T, Okuda H. Physicochemical properties and in vitro intestinal permeability properties and intestinal cell toxicity of silica particles, performed in simulated gastrointestinal fluids. Biochim Biophys Acta. 2014;1840:1171–80.
Gelli R, Tempesti P, Ridi F, Baglioni P. Formation and properties of amorphous magnesium-calcium phosphate particles in a simulated intestinal fluid. J Colloid Interface Sci. 2019;546:130–8.
Jiang X, Zhang X, Gray P, Zheng J, Croley TR, Fu PP, et al. Influences of simulated gastrointestinal environment on physicochemical properties of gold nanoparticles and their implications on intestinal epithelial permeability. J Environ Sci Heal Part C Environ Carcinog Ecotoxicol Rev. 2019;37:116–31.
Gou J, Feng S, Liang Y, Fang G, Zhang H, Yin T, et al. Polyester-solid lipid mixed nanoparticles with improved stability in gastro-intestinal tract facilitated oral delivery of larotaxel. Mol Pharm. 2017;14:3750–61.
Li Z, Ha J, Zou T, Gu L. Fabrication of coated bovine serum albumin (BSA)-epigallocatechin gallate (EGCG) nanoparticles and their transport across monolayers of human intestinal epithelial Caco-2 cells. Food Funct. 2014;5:1278–85.
Ibrahim HM, Awad M, Al-Farraj AS, Al-Turki AM. Stability and dynamic aggregation of bare and stabilized zero-valent iron nanoparticles under variable solution chemistry. Nanomaterials. 2020;10:192.
Park S, Lee WJ, Park S, Choi D, Kim S, Park N. Reversibly pH-responsive gold nanoparticles and their applications for photothermal cancer therapy. Sci Rep. 2019;9:20180.
Asadi E, Azodi-Deilami S, Abdouss M, Khaghani S. Cyproterone synthesis, recognition and controlled release by molecularly imprinted nanoparticle. Appl Biochem Biotechnol. 2012;167:2076–87.
Jannin V, Dellera E, Chevrier S, Chavant Y, Voutsinas C, Bonferoni C, et al. In vitro lipolysis tests on lipid nanoparticles: comparison between lipase/co-lipase and pancreatic extract. Drug Dev Ind Pharm. 2015;41:1582–8.
Hosseinidoust Z, Alam MN, Sim G, Tufenkji N, van de Ven TGM. Cellulose nanocrystals with tunable surface charge for nanomedicine. Nanoscale. 2015;7:16647–57.
Wang J, Zhang L, Peng F, Shi X, Leong DT. Targeting endothelial cell junctions with negatively charged gold nanoparticles. Chem Mater. 2018;30:3759–67.
Schleh C, Semmler-Behnke M, Lipka J, Wenk A, Hirn S, Schäffler M, et al. Size and surface charge of gold nanoparticles determine absorption across intestinal barriers and accumulation in secondary target organs after oral administration. Nanotoxicology. 2012;6:36–46.
Walczyk D, Bombelli FB, Monopoli MP, Lynch I, Dawson KA. What the cell “sees” in bionanoscience. J Am Chem Soc. 2010;132:5761–8.
Kumar S, Yadav I, Aswal VK, Kohlbrecher J. Structure and interaction of nanoparticle-protein complexes. Langmuir. 2018;34:5679–95.
Ranjan S, Dasgupta N, Sudandiradoss C, Ramalingam C, Kumar A. Titanium dioxide nanoparticle-protein interaction explained by docking approach. Int J Nanomed. 2018;13:47–50.
Bhogale A, Patel N, Sarpotdar P, Mariam J, Dongre PM, Miotello A, et al. Systematic investigation on the interaction of bovine serum albumin with ZnO nanoparticles using fluorescence spectroscopy. Colloids Surf B Biointerfaces. 2013;102:257–64.
Sasidharan A, Chandran P, Monteiro-Riviere NA. Biocorona bound gold nanoparticles augment their hematocompatibility irrespective of size or surface charge. ACS Biomater Sci Eng. 2016;2:1608–18.
Lundqvist M, Stigler J, Cedervall T, Berggård T, Flanagan MB, Lynch I, et al. The evolution of the protein corona around nanoparticles: a test study. ACS Nano. 2011;5:7503–9.
Maiorano G, Sabella S, Sorce B, Brunetti V, Malvindi MA, Cingolani R, et al. Effects of cell culture media on the dynamic formation of protein-nanoparticle complexes and influence on the cellular response. ACS Nano. 2010;4:7481–91.
Tsoi KM, MacParland SA, Ma X-Z, Spetzler VN, Echeverri J, Ouyang B, et al. Mechanism of hard-nanomaterial clearance by the liver. Nat Mater. 2016;15:1212–21.
Yu M, Song W, Tian F, Dai Z, Zhu Q, Ahmad E, et al. Temperature- and rigidity-mediated rapid transport of lipid nanovesicles in hydrogels. Proc Natl Acad Sci U S A. 2019;116:5362–9.
Choki K, Li S, Ye A, Jameson GB, Singh H. Fate of hydroxyapatite nanoparticles during dynamic in vitro gastrointestinal digestion: the impact of milk as a matrix. Food Funct. 2021;12:2760–71.
Levak M, Burić P, Dutour Sikirić M, Domazet Jurašin D, Mikac N, Bačić N, et al. Effect of protein corona on silver nanoparticle stabilization and ion release kinetics in artificial seawater. Environ Sci Technol. 2017;51:1259–66.
Martin MN, Allen AJ, MacCuspie RI, Hackley VA. Dissolution, agglomerate morphology, and stability limits of protein-coated silver nanoparticles. Langmuir. 2014;30:11442–52.
Chao Y, Marsh AI, Behray M, Guan F, Engdahl A, Chao Y, et al. Synthesis and characterisation of isothiocyanate functionalised silicon nanoparticles and their uptake in cultured colonic cells. Faraday Discuss. 2020;222:332–49.
Marchiando AM, Graham WV, Turner JR. Epithelial barriers in homeostasis and disease. Annu Rev Pathol. 2010;5:119–44.
Van Spaendonk H, Ceuleers H, Witters L, Patteet E, Joossens J, Augustyns K, et al. Regulation of intestinal permeability: the role of proteases. World J Gastroenterol. 2017;23:2106–23.
Brun E, Barreau F, Veronesi G, Fayard B, Sorieul S, Chanéac C, et al. Titanium dioxide nanoparticle impact and translocation through ex vivo, in vivo and in vitro gut epithelia. Part Fibre Toxicol. 2014;11:13.
Cao X, Khare S, DeLoid GM, Gokulan K, Demokritou P. Co-exposure to boscalid and TiO(2) (E171) or SiO(2) (E551) downregulates cell junction gene expression in small intestinal epithelium cellular model and increases pesticide translocation. NanoImpact. 2021;22:100306.
Zhang Y, Duan S, Liu Y, Wang Y. The combined effect of food additive titanium dioxide and lipopolysaccharide on mouse intestinal barrier function after chronic exposure of titanium dioxide-contained feedstuffs. Part Fibre Toxicol. 2021;18:8.
Lee Y, Kamada N, Moon JJ. Oral nanomedicine for modulating immunity, intestinal barrier functions, and gut microbiome. Adv Drug Deliv Rev. 2021;179:114021.
Tang M, Li S, Wei L, Hou Z, Qu J, Li L. Do engineered nanomaterials affect immune responses by interacting with gut microbiota? Front Immunol. 2021;12:684605.
Goto Y. Epithelial cells as a transmitter of signals from commensal bacteria and host immune cells. Front Immunol. 2019;10:2057.
Colombo G, Cortinovis C, Moschini E, Bellitto N, Perego MC, Albonico M, et al. Cytotoxic and proinflammatory responses induced by ZnO nanoparticles in in vitro intestinal barrier. J Appl Toxicol. 2019;39:1155–63.
Busch M, Bredeck G, Kämpfer AAM, Schins RPF. Investigations of acute effects of polystyrene and polyvinyl chloride micro- and nanoplastics in an advanced in vitro triple culture model of the healthy and inflamed intestine. Environ Res. 2021;193: 110536.
Kokalari I, Gassino R, Giovannozzi AM, Croin L, Gazzano E, Bergamaschi E, et al. Pro- and anti-oxidant properties of near-infrared (NIR) light responsive carbon nanoparticles. Free Radic Biol Med. 2019;134:165–76.
Tyanova S, Temu T, Cox J. The MaxQuant computational platform for mass spectrometry-based shotgun proteomics. Nat Protoc. 2016;11:2301–19.
Tyanova S, Temu T, Sinitcyn P, Carlson A, Hein MY, Geiger T, et al. The Perseus computational platform for comprehensive analysis of (prote)omics data. Nat Methods. 2016;13:731–40.
Sambuy Y, De Angelis I, Ranaldi G, Scarino ML, Stammati A, Zucco F. The Caco-2 cell line as a model of the intestinal barrier: influence of cell and culture-related factors on Caco-2 cell functional characteristics. Cell Biol Toxicol. 2005;21:1–26.
Dussert F, Wegner KD, Moriscot C, Gallet B, Jouneau P-H, Reiss P, et al. Evaluation of the dermal toxicity of InZnP quantum dots before and after accelerated weathering: toward a safer-by-design strategy. Front Toxicol. 2021;3:6.
Konishi Y, Hagiwara K, Shimizu M. Transepithelial transport of fluorescein in Caco-2 cell monolayers and use of such transport in in vitro evaluation of phenolic acid availability. Biosci Biotechnol Biochem. 2002;66:2449–57.
Balivada S, Rachakatla RS, Wang H, Samarakoon TN, Dani RK, Pyle M, et al. A/C magnetic hyperthermia of melanoma mediated by iron(0)/iron oxide core/shell magnetic nanoparticles: a mouse study. BMC Cancer. 2010;10:119.
Jeitner TM. Optimized ferrozine-based assay for dissolved iron. Anal Biochem. 2014;454:36–7.
ANalisys Of VAriance. p. https://astatsa.com/OneWay_Anova_with_TukeyHSD/.
The Authors thank Mr. Costanzo Costamagna, Department of Oncology, University of Torino, for the technical assistance and Dr. Marta Vassallo for her contribution in some investigations.
This research has received funding by the European Union’s Horizon 2020, Research and Innovation Program “BIORIMA”, under Grant Agreement No. 760928.
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Additional file 1.
Figure S1. Optical appearance of the colloidal suspensions before A) and after B) treatment with the SHDS. Figure S2. Size distribution of the samples directly incubated in SIF or after complete SHDS-treatment of A) LSNPs; B) CNPs, C) FNPs; D) HNPs. Figure S3. HNPs dissolution. Figure S4. Degradation of LSNPs by lipase. Table S1. Mean dH and PDI of NMs in DMEM+10% FBS (100 mg/ml), 24 h incubation. Figure S5. Aspect of the suspension of the (*) untreated and (**) SHDS-treated A) LSNPs, B) CNPs, C) FNPs and D) HNPs in cell medium. Figure S6. SDS-PAGE analysis showing the hard corona of (*) SHDS-treated and (**) untreated A) LSNPs, B) CNPs, C) FNPs and D) HNPs in cell medium and obtained by centrifugation, and E) ctrl without NBMs. Figure S7. LFQ intensity for different proteases inhibitor for FNPs untreated and SHDS-treated. Figure S8. Cells viability of A) Caco-2 cells and B) HCoEpiC cells after 24 h of incubation with SHDS fluids. Figure S9. Genotoxicity of HCT116 cells after 24 h of incubation with untreated and SHDS-treated NMs. Table S2. Tran-Epithelial Electrical Resistance (TEER) values of Caco-2 barrier model after 24 h of incubation. Figure S10. Scheme of representative SDHS treatment.
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Antonello, G., Marucco, A., Gazzano, E. et al. Changes of physico-chemical properties of nano-biomaterials by digestion fluids affect the physiological properties of epithelial intestinal cells and barrier models. Part Fibre Toxicol 19, 49 (2022). https://doi.org/10.1186/s12989-022-00491-w
- In vitro simulated digestion
- Gastro-intestinal barrier