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Shiga Toxin-B Targeted Gold Nanorods for Local Photothermal Treatment in Oral Cancer Clinical Samples

Authors Navarro-Palomares E, García-Hevia L , Galán-Vidal J , Gandarillas A, García-Reija F, Sánchez-Iglesias A, Liz-Marzán LM, Valiente R , Fanarraga ML 

Received 12 July 2022

Accepted for publication 3 October 2022

Published 28 November 2022 Volume 2022:17 Pages 5747—5760

DOI https://doi.org/10.2147/IJN.S381628

Checked for plagiarism Yes

Review by Single anonymous peer review

Peer reviewer comments 4

Editor who approved publication: Prof. Dr. Anderson Oliveira Lobo



Elena Navarro-Palomares,1 Lorena García-Hevia,1 Jesús Galán-Vidal,2 Alberto Gandarillas,2 Fe García-Reija,3 Ana Sánchez-Iglesias,4,5 Luis M Liz-Marzán,4,5 Rafael Valiente,1,6 Mónica L Fanarraga1

1The Nanomedicine Group, Valdecilla Health Research Institute IDIVAL, Universidad de Cantabria, Santander, 39011, Spain; 2Cell Cycle, Stem Cell Fate & Cancer Laboratory, Valdecilla Health Research Institute IDIVAL, Santander, 39011, Spain; 3Oral and Maxillofacial Surgery Unit, Valdecilla Hospital HUVM, Santander, Spain; 4CIC biomaGUNE, Basque Research and Technology Alliance (BRTA), and CIBER de Bioingeniería, Biomateriales y Nanomedicina (CIBER-BBN), San Sebastián, 20014, Spain; 5Ikerbasque, Basque Foundation for Science, Bilbao, 48009, Spain; 6Dpt. Applied Physics, Facultad de Ciencias, Universidad de Cantabria, Santander, 39005, Spain

Correspondence: Mónica L Fanarraga; Lorena García-Hevia, Valdecilla Health Research Institute IDIVAL, University of Cantabria, Avda Herrera Oria s/n, Santander, 39011, Spain, Tel +34 942315515 Ext. 74101, Email [email protected]; [email protected]

Introduction: A great challenge in nanomedicine, and more specifically in theranostics, is to improve the specificity, selectivity, and targeting of nanomaterials towards target tissues or cells. The topical use of nanomedicines as adjuvants to systemic chemotherapy can significantly improve the survival of patients affected by localized carcinomas, reducing the side effects of traditional drugs and preventing local recurrences.
Methods: Here, we have used the Shiga toxin, to design a safe, high-affinity protein-ligand (ShTxB) to bind the globotriaosylceramide receptor (GB3) that is overexpressed on the surfaces of preneoplastic and malignant cancer cells in the head and neck tumors.
Results: We find that ShTxB functionalized gold nanorods are efficiently retrotranslocated to the GB3-positive cell cytoplasms. After 3 minutes of laser radiation with a wavelength resonant with the AuNR longitudinal localized surface plasmon, the death of the targeted cancer cells is activated. Both preclinical murine models and patient biopsy cells show the non-cytotoxic nature of these functionalized nanoparticles before light activation and their treatment selectivity.
Discussion: These results show how the use of nanomedicines directed by natural ligands can represent an effective treatment for aggressive localized cancers, such as squamous cell carcinoma of the oral cavity.

Keywords: functionalized nanomaterial, natural ligand, nanoparticle targeting, squamous carcinoma, globotriaosylceramide

Introduction

Nanomedicine has ushered in a new era in drug delivery, improving drug stability and targeting, while reducing biodegradation. However, targeting nanomaterials efficiently to tissues and controlling their intracellular fate are among the major issues in nanomedicine, resulting in that low success in the `bench-to-bed´ translation. As with chemotherapy, it is estimated that less than 1% of systemically administered nanomedicines reach the tumor stroma.1–4 Hence, nanomaterials’ low targeting efficiency and potential toxicity are considered a double-edged sword that limits their application.

To improve the specificity, biocompatibility, and selectivity of nanomedicines, nanomaterials are functionalized through surface modifications. Most nanotherapies under development are based on the conjugation of nanoparticles with antibodies,5 or fragments thereof,6 for their specific targeting to receptors on tumor cells, to which they bind with high affinity.7 However, nanoparticle instability, the limited penetration into tissues, and the inability to cross cell membranes are the main disadvantages.8 As a consequence, drug concentrations administered to tumor cells do not reach threshold therapeutic doses and may even generate resistance.9 But, until the targeting of systemically administered nanomaterials improves, nanomedicine could have enormous potential in the local treatment of accessible cancers, especially those that have imprecise borders or cause recurrences of adjacent neoplastic cells.

In this scenario, virus and toxin recognition mechanisms offer an interesting alternative. These natural systems have evolved over millions of years to perfect their targeting, cell entry, and infection mechanisms binding specific receptors with nanomolar affinities.10,11 Besides, they efficiently manipulate the response of their host cells using simple molecular cues that trigger programmed cellular behaviors. Interestingly, some of the cell entry mechanisms used by these natural systems can also circumvent the receptor-mediated `canonical´ endo-lysosomal entry route to prevent their degradation or exocytosis.

In the search for new receptor-mediated cell entry routes bypassing the canonical endo-lysosomal vesicular pathway, we decided to investigate the Shiga toxin (ShTx) as a protein-ligand.12 This toxin, produced by Shigella dysenteriae and certain strains of Escherichia coli, is a protein that specifically recognizes globotriaosylceramide (GB3 or CD77).13 The mechanism of ShTx cell recognition and invasion is one of the most well-known systems of prokaryotic hijacking of eukaryotic response.14 The toxin penetrates the cytoplasm of the target cells bypassing the endolysosomal pathway, thus avoiding exposure to enzymatic and acid lysosomal media that would destroy the toxin and, in our case, the therapeutic agents.15 Interestingly, several studies have localized the ShTx receptor in cancer cells of different origins.13,16–20 This glycosphingolipid, enriched in membrane microdomains known as lipid rafts, is overexpressed in many multidrug-resistant human tumor cells and is, therefore, a very interesting receptor for the treatment of malignant neoplasms.

Among all localized and accessible cancers, we have focused on squamous cell carcinoma head and neck (HNC). This includes a great heterogeneity of tumors that arise from the mucosal surfaces of the oral cavity, that are difficult to treat, and are typically characterized by recurrences that are often fatal. Indeed, this is the sixth most common form of cancer,21,22 with survival rates of approximately 40–50% five years after diagnosis.23,24 This cancer is generally removed surgically and then treated with adjuvant radiotherapy or chemoradiotherapy.21 However, fatal recurrences are very common due to poor detection of preneoplastic areas, deficient removal of the affected tissue, and poor penetration of the systemic drug into the tumoral mass.

We believe HNC is a clear example of a heterogeneous localized malignancy that could significantly benefit from the local treatment with targeted nanomedicines for both, diagnosis and treatment. Interestingly, previous studies have established that GB3 is a marker for preneoplastic and malignant HNC cells.18 Thus, given that this type of cancer allows the topical application of nanomaterials, our hypothesis is to use nanoparticles directed by ShTxB as a local treatment to avoid possible systemic toxicity. In this study, we genetically engineered an innocuous ShTx-based ligand protein for conjugation with gold nanorods (AuNRs) to identify and kill preneoplastic and malignant HNC cells by local photohyperthermia.

Materials and Methods

Gene Synthesis, Protein Expression, and Purification

ShTxB:6xHis recombinant gene construct was synthesized by General Biosystems, Inc. (Morrisville, USA) (Figure S1) and was cloned in pET-15b plasmid systems (Novagen, Merck KGaA, Spain). One Shot™ BL21 (DE3) E. coli (NZYTech, Portugal) cells were transformed with the expression vector. Bacterial cultures were grown in Luria-Bertani (LB) broth supplemented with 100 μg/mL ampicillin and 35 μg/mL chloramphenicol until A600 ca. 0.6. The expression of the protein was induced by adding 0.1 mM isopropyl b-D thiogalactopyranoside (IPTG). Cells were collected after 4 hours by centrifugation and were resuspended in 50 mM NaPi, 300 mM NaCl, pH 8.0 with 1 mg/mL lysozyme, and protease inhibitors (Pierce, Thermo Fischer, Spain).

Bacterial cell lysates were obtained by probe sonication (5 × 15s pulses at 130 W, 65% amplitude, with 15s intervals, at 4℃), and insoluble material was removed by centrifugation. Bacterial soluble protein lysate was loaded onto pre-equilibrated Ni-TED columns (Protino® Ni-TED, Macherey-Nagel GmbH & Co., Düren, Germany). The recombinant His-tagged protein was eluted in a buffer supplemented with 250 mM imidazole. Finally, PD-10 desalting Columns (GE Healthcare, Chicago, USA) were used to remove the imidazole and to exchange buffer for PBS.

Nanorods Synthesis, SiO2 Coating, and Characterization

Gold nanorods (AuNRs) in CTAB (Cetyltrimethylammonium Bromide) were synthesized using salicylic acid as an additive as previously described.25,26 For coating AuNRs with silica, CTAB on the surface was exchanged with mPEG-SH. Excess CTAB was washed by repeated centrifugation, AuNRs were resuspended in Milli-Q water and a solution of mPEG-SH (50 molecules/nm2) was added dropwise. After 1 h of stirring AuNRs were washed and finally redispersed in ethanol. Silica coating was performed by mixing AuNRs ([Au] = 0.5 mM) with the appropriate amount of H2O (10.55 M), NH3 (0.2M), and tetraethyl orthosilicate (TEOS) solution (1 mM) and allowing reaction for 6 h at room temperature (RT).27 The fluorophore Rhodamine B isothiocyanate (RBITC) was conjugated to APMS and added in subsequent shell re-growth steps allowing its conjugation to SiO2.28 Fluorescently coated AuNRs were washed by repeated cycles of centrifugation/redispersion in ethanol. All reagents were obtained from Sigma-Aldrich, except ethanol (96%) which was purchased from Scharlab. Ethanol-dispersed nanorods were adsorbed onto a Lacey copper grid (400 mesh, EM Resolutions) and characterized using a JEM 1011 (JEOL) transmission electron microscope (TEM)(Figure S2).

Protein Bioconjugation on Particles, SDS-PAGE Protein Analysis

Nanorods were functionalized with 0.5 mg/mL of the protein solution (saturating amounts) in PBS during 3×2 s mild sonication at RT. For SDS-PAGE, the protein functionalized on the particles was stripped using Laemmli sample buffer 1× (BioRad) at 90 °C for 2 min. SDS-PAGE electrophoresis was performed using Mini-Protean® precast gels (BioRad). Protein analysis was performed on Coomassie blue-stained gels that were scanned using the BioRad GelDoc EZ system.

Cell Culture and Compacted Pellet (Micro Tumor) Conditions

Detroit 562 cells, human pharynx epithelial carcinoma cells derived from a metastatic pleural effusion, and MCF-7, human breast cancer cells, were obtained from ATCC Ref. CCL-138 and HTB-22 respectively. Detroit 562 cells were grown in Modified Eagle´s Medium and MCF-7 cells in Dulbecco´s Modified Eagle´s Medium (Sigma) containing 10% bovine serum. Both cell lines were kept in standard conditions. MCF7 cells were used as controls (GB3-ve) after characterization with the anti-GB3 antibody (Figure S4). A total of 500.000 cells were washed, trypsinized, and centrifuged at 1000 rpm for 5 minutes. The supernatant was removed, and pellets were re-suspended in 50 μL of culture media to create a cell pellet that was used as a microtumor.

Staining, Fluorescent, and Electron Microscopy Imaging

Cells were exposed to 5 µg/mL of bioconjugated [email protected]2:[email protected] particles for 3 hours. Cells were fixed with 4% paraformaldehyde, were stained with Hoechst 33258 (Sigma-Aldrich®), Acridine Orange (Sigma-Aldrich®) for live cells, or ethidium bromide (Sigma) for dead cells. Alexa647-anti-Human CD77 (BD Pharmingen™, UK) was used for immunostaining the GB3 receptor. Confocal images were taken with a Nikon A1R microscope. All fluorescent images are pseudo-colored. Cell samples processed for electron microscopy were fixed with 3% glutaraldehyde in 0.12 M PBS for 24 hours and were post-fixed in 2% buffered osmium tetroxide, dehydrated in a graded acetone series, and embedded in Araldite. Ultrathin sections of ca. 70 nm thick, were obtained on an LKB ultramicrotome, stained with lead citrate and uranyl acetate. TEM was performed using a JEOL JEM 1011 operated at 100 kV.

Flow Cytometry

Cell death quantification experiments were performed with a total of 106 Detroit and MCF-7 cells. Cells were stained with Annexin V-FITC kit (Immunostep) for 15 min. and then passed through the cytometer (CytoFLEX, Beckman Coulter). Quantitative GB3 expression was validated and measured in a total of 10.000 Detroit and MCF-7 cells immunostained with Alexa647-anti-Human CD77 (BD Pharmingen™, UK) for 30 minutes and then fixed in 4% paraformaldehyde (Figure S4). Qualitative interaction of [email protected]2@ShTxB in cells was performed using 10.000 Detroit 562 and MCF-7 cells. Cells were exposed to the nanoparticles for 3h, washed, and passed through the cytometer. Data were analyzed using the CytExpert software.

Murine Model and Tissue Processing

In vivo experiments were designed and performed to minimize the use of animals. Ethical permissions for this study were requested, approved, and obtained from the Bioethics Committee University of Cantabria, General Directorate of Livestock, Government of Cantabria (Project Ref PI-11-21). C57BL/6 mice (12 weeks old female/male of 20–25mg of weight) were housed with a 12 h light/dark cycle with free provision of food and water at the Experimentation Service (SEEA) of the University of Cantabria. The animals were maintained, handled, and sacrificed following the directive 2010/63/UE. The preclinical model of oral carcinogenesis was produced using the carcinogen 4-Nitro-quinoline-1-oxide (4-NQO, Sigma Aldrich) as previously described.29–31 In brief, 12 mice were offered drinking water with 100 μg/mL of 4-NQO for 16 weeks (water was changed once a week). After 16 weeks of the treatment, the mice with visible lesions in the oral cavity were treated with 5 µg/mL of [email protected]2@ShTxB in the drinking water (approximately 1 mg/kg mice total) for 24 hours before sacrifice. For the laser irradiation, 6 mice were humanely sacrificed and the tissues were dissected and immediately irradiated as indicated in the text. The irradiation procedure was performed only once. The tissues were fixed in 10% formalin, embedded in paraffin, sectioned (4 μm thick), deparaffinized, stained with hematoxylin-eosin, or preserved in optimal cutting temperature compound (OCT) at −80℃ to be cryosectioned. Approximately 6 μm cryostat sections were fixed in paraformaldehyde 4%, immunostained with Alexa 647-anti-Human CD77 (BD Pharmingen™, UK), and with Hoechst.

Human Biopsies and Cell Culture of Head and Neck Squamous Carcinoma Cells

Ethical permissions for this study were requested, approved, and obtained from the Ethical Committee for Clinical Research of Cantabria Council, Spain (Ref. 2017.259). The study complies with the Declaration of Helsinki. In all cases, human tissue material discarded after surgery was obtained with written consent presented by clinicians to the patient and was treated anonymously. Biopsy sample cell cultures were grown from biopsies of malignancies localized at the floor of the mouth (MASCC, moderately aggressive, intermediate grade), and retromolar trigone (ASCC, high grade, aggressive). The grade of aggressiveness was characterized by the clinician. Control cells were isolated from a healthy human biopsy (cheek inner mucosa). Biopsies were cut into pieces and washed twice with PBS‐EDTA, 100 U/mL penicillin‐streptomycin (Pen/Strep), and 0.5 μg/mL Amphotericin B. Pieces were then washed twice with 1x PBS, 100 U/mL Pen/Strep, and 0.5 μg/mL Amphotericin B and incubated with agitation at 37 °C for 4 rounds of 15 min with 0.075% trypsin, 2.5 mg/mL collagenase P, 1× PBS, 100U/mL Pen/Strep and 0.5 μg/mL Amphotericin B. Isolated keratinocytes were co-cultured with a feeder layer of (3T3)-J2 mouse fibroblast feeder layer (previously inactivated with mitomycin C).

HNSCC and healthy primary keratinocytes were cultured in a modified Rheinwald FAD medium.32,33 3:1 v/v Dulbecco’s Modified Eagle Medium – Ham’s F12, 5% fetal bovine serum, 0.5 μg/mL hydrocortisone, 5 ng/mL epidermal growth factor, 9 ng/mL cholera toxin, 1.8×10−4 M adenine, 5 µg/mL insulin, 2 mM L‐glutamine, 0.75 mM sodium pyruvate, and 100 U/mL Pen/Strep. Mouse fibroblast 3T3-J2 cell line used as feeder layer was cultured in Dulbecco medium with 10% donor calf serum and 100 U/mL Pen/Strep.

Laser Microtumor Irradiation

Detroit 562 and control MCF-7 cells were exposed to 5 µg/mL and 10 µg/mL of [email protected]2@ShTxB for 3h. Then cells were washed, pelleted into microtumors, and irradiated with an unfocused NIR laser (808 nm LD, 1 W) for 10 min. After irradiation cells were placed back in culture plates in the incubator for another 24 hours. After this period, cells were stained with a dead cell apoptosis kit with AnnexinV-FITC and PI, for flow cytometric analysis and confocal microscopy at 0 and 24h.

Laser Irradiation

Cultures of neoplastic or normal cells from oral biopsies cells were treated with 5 µg/mL [email protected]2@ShTxB for 3 h. After removal of the particles in the media, cultures were irradiated with the 808 nm LD for 10 min directly on the plate. In vivo tumor irradiation: Once verrucous cancerous lesions were visible in the oral cavity, the mice were supplied with water containing 10 μg/mL of the [email protected]2:[email protected] particles for 12h. The mice were euthanized, and the tongues were dissected and photographed. These tissues were irradiated with an 808 nm laser for 5 min. Tissues were then processed and sectioned for analysis.

Statistical Analysis

Student’s t-test statistical analysis was used for statistical analysis and to evaluate significance that was established for a *p < 0.025 or a **p < 0.005. Quantitative results are expressed as mean values with their corresponding standard error bars. These statistical analyses were done using SPSS, version 19.0.

Results

Targeting Ligand Design

The ShTx belongs to the AB5 toxin family secreted by some pathogenic bacteria (Figure 1A).34 All these toxins share a similar structure and follow identical mechanisms for entering the targeted cells. From the structural point of view, ShTx is composed of 6 (1+5) polypeptides (Figure 1A). The “A” subunit is the catalytic subunit that, upon internalization, interferes with the regular functions of the host cell. The rest of the toxin comprises five identical copies of the “B” subunit, which assemble into a homopentamer surrounding the “A” subunit. Each “B” subunit can contact the receptor on the target cell membrane by triggering clustering upon coupling, thereby provoking membrane ruffling.12,34–37

Figure 1 (A) Shiga toxin (ShTx) structure. The predicted structure of the engineered ShTxB-like ligand-protein. A single B domain (ShTxB) (blue) is attached to the 6xHis cationic tail (red). (B) TEM images of AuNRs before and after SiO2 coating. (C) Diagram of the synthetic steps for production of [email protected]2@ShTxB. Created with BioRender.com. (D) Coomassie-stained SDS-PAGE gels showing (#1) Recombinant ShTxB-ligand protein overexpression, (#2) purified ShTxB, and (#3) ShTxB stripped from the functionalized [email protected]2@ShTxB.

The ShTx “B” subunits are innocuous high-affinity GB3 natural ligands12,38 that have been used to successfully drive fluorophores,39,40 radionuclides,41 drugs,16,42 or even nanoparticles17 to the cytoplasm of GB3 positive (GB3+ve) cells. Given these results, we proposed to use this fragment of the ShTx protein as a ligand to target multifunctional photoactivatable nanomaterials to GB3 positive (GB3+ve) squamous carcinoma cells.

To remove the catalytic part of the protein, and prevent nonspecifically cell death, we genetically engineered a new protein that contained only the toxin receptor-binding domain B. This toxin fragment was genetically fused to a cationic peptide. This allows the electrostatic functionalization with the negative surface of the silica-coated particles as previously described.17,43 Furthermore, this method allows positioning the ligand-domain of the protein correctly oriented on the nanoparticle surface (Figure 1A).43 Besides, this functionalization method also reduces the non-specific protein biofouling and it is very stable upon exposure to physiological conditions (> 72 h).43 The designed chimera protein named ShTxB:6xHis (hereafter ShTxB) containing the ShTx “B” subunit (UniProtKB ref. P09386) was genetically linked to its C-terminus to a hexahistidine tag (6xHis). The ShTxB protein was overexpressed for production in bacteria and purified using affinity columns (Experimental Section) (Figure S1).

AuNRs Synthesis and Functionalization

To destroy the cancer cells topically we designed nanomaterials capable of producing hyperthermia upon laser illumination. Among the wide variety of available plasmonic nanomaterials, AuNRs are arguably the most commonly used system,44 on account of their reproducible and versatile synthesis methods, and tunable localized surface plasmon resonances (LSPR).45 For the present study, we synthesized AuNRs with dimensions of ca. 55 nm x 13 nm (Figures 1B and S2), resulting in a longitudinal LSPR band centered at 803 nm, resonant with an 808 nm laser diode, within the first biological window. Details of the synthesis protocol can be found elsewhere.44 For in cellulo localization purposes, AuNRs were coated with a ca. 35 nm thick Rhodamine B isothiocyanate (RBITC) stained amorphous silica shell ([email protected]2) (Figure 1B), prepared following the procedure described previously.28 Before activation, the resulting [email protected]2:RBTIC particles displayed no detectable toxicity at 5–15 µg/mL dosages when applied to human pharynx epithelial carcinoma after 96 h (Figure S3).

The design was finalized by biofunctionalization of the [email protected]2:RBTIC with an ShTxB ligand-protein layer (Figure 1C). Bioconjugation of the nanoparticles was done by incubation in a 0.5 mg/mL solution of ShTxB:6xHis protein produced in bacteria and subsequently purified following standard procedures (see details in the Supplementary Information). The presence of ShTxB on the [email protected]2:RBTIC surface was biochemically validated by SDS-PAGE analysis (Figure 1D and S1B).

Affinity of the ShTxB Functionalized AuNRs for HNC Cells

To determine the affinity of the functionalized [email protected]2:[email protected] for HNC cells bearing the GB3 receptor we chose Detroit 562 cells from human pharynx epithelial carcinoma derived from a metastatic pleural effusion. As negative controls, we used MCF-7 human breast cancer cells lacking the GB3 receptor (GB3-ve). Confirmation of the presence/absence of the receptor in both cell models was investigated by immunostaining with anti-GB3 antibodies using two technologies, flow cytometry and confocal microscopy (Figure S4). Upon validation of the models, we tested the affinity of the nanoconjugates for the neoplastic cells. To do this, 2D cultures of the two cell types were exposed in parallel to 5 µg/mL of nanoparticles functionalized with ShTxB in culture media for 2 h. At this time, the cells were fixed and processed for flow cytometry for quantification of the captured functionalized nanorods (Figure 2A). We found that, compared to controls (<2% cells containing nanorods), more than 90% of HNC GB3+ve cells (Detroit 562) captured nanoparticles during this incubation period. This finding was next validated using confocal microscopy. Figure 2B shows how, two 2h after nanoparticle incubation with the cells, the nanorods co-localized with the cytoplasmic membrane presumably coupled with clustered GB3 receptors (orange arrows). This result was also supported by TEM images of ultrathin sections of the cells (Figure 2C and D). Together, these data support the hypothesis that ShTxB-coated nanorods efficiently interact with GB3 receptors on HNC cells penetrating the cellular cytoplasm of these neoplastic cells (Figure 2D).

Figure 2 [email protected]:[email protected] cell selectivity. (A) Flow cytometry quantification of the interaction of [email protected]2:[email protected] with control (GB3-ve) and HNC (GB3+ve) cells. Cells were exposed to the nanoparticles for 2 h and then washed before fixation and flow cytometry analysis. Created with BioRender.com. (B) Confocal microscopy single Z-plane image of human HNC neoplastic cells exposed to 5 µg/mL of the [email protected]2:[email protected] (red channel) and live immunostained for GB3 (green channel). Clustered nanorods colocalize with GB3 receptors on the cell surface (Orange arrows). (C and D) TEM images of ultrathin sections of HNC neoplastic cells incubated with [email protected]2:[email protected] The AuNRs contact the cell surface (red arrow). (C) Engulfed particles appear in large irregular membranous structures close to the cell edge or the cytosol in the proximity to cytoplasmic membranes. Some AuNRs can be observed free in the cytosol (white arrow). (D) Image of a whole GB3+ve HNC cell where the functionalized nanoparticles can be found both, in a membranous structure (empty arrow), or free in the cytoplasm (filled arrow).

Photohyperthermia to Destroy HNC Cells

The morphology of the AuNRs was designed to induce heating by illumination with an LD of 808 nm, coinciding with the first biological window. For these studies, HNC cells were exposed to [email protected]2@ShTxB for 2 h, were washed, and then collected into pellets of approximately 2 mm roughly resembling solid microtumors, (see the experimental design in Figure 3A). These were irradiated for 3 or 10 min with an unfocused 1 W fiber LD at 808 nm, in resonance with the longitudinal LSPR of AuNRs. After irradiation, cells were immediately reseeded and allowed to grow for 24 h before live/dead quantification by flow cytometry (Figure 3A).

Figure 3 Selective elimination of HNC cancer cells with [email protected]2@ShTxB after irradiation. (A) Diagram of the experimental procedure. Created with BioRender.com. (B) Live / dead cell quantification 24h after irradiation in control (GB3-ve), and HNC (GB3+ve) cells by AnnexinV-FITC/PI staining and flow cytometry (Figure S4). Dead cells appear in the upper right frame of the chart. (C) Average percentages of cell viability upon LD irradiation to microtumors (approx. 10,000 cells measured per experiment; n = 3; *For a *p < 0.025 or a ***p < 0.005.

The study revealed that a 3-minute laser exposure was sufficient to kill ca. 50% of GB3+ve neoplastic cells that contained [email protected]2@ShTxB (Figure 3B). Longer irradiation periods (10 min) eliminated ca. 80% of the HNC cells (Figure 3C). In contrast, control GB3-ve cells treated in parallel were almost unaffected by exposure to nanomaterials and laser radiation. (Figure 3B).

As a complement, we also investigated this effect in 2D multilayered cultures of HNC neoplastic cells. Following the experimental depicted in Figure 4A, we incubated cultures of Detroit 562 cells with [email protected]2@ShTxB (5 µg/mL for 3 h) and exposed the cultures to an 808 nm unfocused laser irradiation for 10 min. Figure 4B shows how, approximately 1 h after irradiation, dead cells (stained in red) appear in the treated area (yellow circle). Dead cells progressively detach from the culture substrate, leaving a clearly visible cell-free area 24 h after irradiation. The delay in the onset of cell death suggested the activation of death cascade processes triggered from the inside out, suggesting apoptosis (see Figure 3B). This process of cell death is more desirable than the necrosis that is normally triggered when cells are abruptly destroyed with heat using external sources or when nanoparticles pierce the cytoplasmic membrane. As expected, no cell death was detected in cultures irradiated without nanoparticles or treated with nanoparticles but not laser (Figure S5A). In the experiment, the temperature in the culture medium was measured during irradiation and no significant changes were observed (Figure S5B). In summary, these results demonstrate that AuNRs functionalized with the ligand-protein ShTxB produce a potent and highly selective cytotoxic effect on HNC cells after laser treatment.

Figure 4 Elimination of cancer cells treated with [email protected]2@ShTxB after irradiation in 2D cultures. (A) Diagram of the experimental procedure. Created with Biorender.com. (B) Cultures of GB3+ve HNC cells stained with acridine Orange (green channel) treated with the [email protected]2@ShTxB and exposed to LD irradiation for 10 min (yellow circle). Cells were cultured for the indicated times before live-dead staining. Dead cells (red) are already visible 1 h after irradiation. The detachment of the dead cells from the culture matrix is evident after 24 h.

Photothermal Effect of ShTxB Functionalized AuNRs in vivo

To assess whether this treatment could be transferred to the clinic, we moved on to preclinical models of study. To do this, we reproduced a well-established squamous cell carcinoma murine model that has been validated in many previous HNC studies using the carcinogen 4-NQO (Supplementary Information).29–31 Treatment of mice with this substance in the drinking water generates visible squamous cell carcinoma lesions on the surfaces of the tongues of the treated mice. Once the tumors were visible, mice were treated with [email protected]2:[email protected] resuspended in drinking water for 24 h. (please see the experimental design in Figure 5A).

Figure 5 (A) Diagram of murine 4-NQO squamous carcinoma preclinical model and summary of the treatment with [email protected]2@ShTxB, followed by photothermal treatment. (B) Post-mortem murine tongues. Blue solid arrows point to representative carcinoma lesions. Empty blue arrows show the same areas after irradiation with an 808 nm LD. These tissues show whiter and swollen lesions. Hematoxylin-eosin-stained sections (H&E) show a patent keratosis at the tongue surface (white arrow) that is visibly affected after the irradiation treatment (black arrows) (bottom row). Similar sections immunostained with anti-GB3 antibody (red channel). Healthy epithelium does not present GB3 immunostaining (red channel) whereas tissues from affected animals show a significantly thickened GB3+ve cornified cell layer. The thickness of the GB3+ve layer cells layer is significantly reduced after a single photothermal treatment (empty white arrows).

For the irradiation, the surfaces of the tongues of the treated mice, that were visibly affected by verrucous and pseudo-hyperplastic carcinomas, were obtained from freshly sacrificed animals. The tongue surfaces were locally irradiated once with a 1 W unfocused LD fiber at 808 nm for 10 min. Irradiation produced some macroscopic changes, indicated with empty blue arrows in Figure 5B. The modifications resulting from this single treatment are more obvious at the microscopic level in tissue sections. Among others, differences in keratosis before (solid white arrow) and after (black arrows) treatment are evident. LD irradiation at 808 nm produced conspicuous destruction on the surface of the warty lesions accompanied by a reduction in the thickness of the GB3+ve cell layer (Figure 5B, empty white arrows). Furthermore, similar to what was observed in cultures treated with nanoparticles and irradiated, the superficial epithelium of the irradiated area was partially detached from the underlying tissues, thus supporting a localized photo-induced hyperthermic effect affecting the GB3+ve zones. These findings suggest that this treatment was effective and that it could be performed repeatedly on the affected area, to destroy the affected GB3+ve neoplastic tissue layer-by-layer until achieving the total elimination of tumor and precancerous cells. Alternatively, the treatment could be applied after surgical removal of the entire tumor to ensure that there are no precancerous areas in the vicinity that could lead to new relapses.

Efficacy of [email protected]2:[email protected] Treatment in Biopsy Samples from Patients Diagnosed with HNC

Finally, we explore the effect of [email protected]2@ShTxB and laser treatment on 3D human cell cultures grown from clinical specimen biopsies of HNC squamous cell carcinomas located on the floor of the mouth (MASCC, moderately aggressive, intermediate grade), and retromolar trigone (ASCC, high grade, aggressive) (Supplementary Information). Control cells were isolated from a healthy human biopsy sample (cheek inner mucosa).

As a preliminary test we first wanted to verify if cells grown from the cancer biopsies were GB3+ve and, secondly, if, as in the cell lines used previously, these cells captured the functionalized nanoparticles. Figure 6 shows how compared to control cells obtained from healthy individuals, cells from the HNC patients displayed abundant GB3 on their surfaces (yellow channel). According to our previous observations, we also found that the HNC biopsy cells internalized a significant amount of [email protected]2:[email protected] nanoparticles into their cytoplasm compared to healthy mucosal cells (red channel).

Figure 6 Confocal microscopy projection images of (A) human control cells (healthy oral tissue) and (B) biopsy cells from human aggressive squamous cell carcinoma (ASCC) cells incubated with 5 µg/mL the [email protected]2:[email protected] (red channel) live immunostained with anti-GB3 antibody (yellow channel). Intracellular clusters of red nanoparticles can be observed inside patients’ cell colonies. Nuclei are stained in blue.

After these preliminary tests, we applied a procedure similar to that described in Figure 4 to these biopsy cell cultures (Figure 7A). For this study, cultures of patients’ cells were exposed to 5 µg/mL of [email protected]2@ShTxB for 2 h. Thereafter, cultures were irradiated for 10 min with 808 nm LD and grown for 24 h before analysis. As seen for cell lines, Figure 7B shows the efficient removal of cancer cells in the culture irradiation area. This treatment, which was highly effective on the cells of the carcinoma sample (MASCC and ASCC), did not affect healthy cells of the oral mucosa treated identically in parallel. No detectable cell death occurred in controls irradiated with the LD but no particles (Figure S6).

Figure 7 (A) Diagram of the experimental procedure for obtaining biopsy sample cell cultures. (B) Live/dead confocal microscopy images of biopsy cells treated with [email protected]2@ShTxB, irradiated with a LD for 10 min and observed immediately (0h), or 24h. Both, the moderately aggressive (MASCC cells) and the aggressive squamous cell carcinoma human cells (ASCC cells) were efficiently eliminated 24 h post after 808 nm LD irradiation. In both cases, the shedding of dead cells in the radiation zone is very evident. Control cells of healthy patients were not affected by the same treatment.

Discussion

The current treatment of choice for this type of tumor is surgery followed by chemotherapy or immunotherapy. Unfortunately, the high mortality of these patients (ca. 50% in the 5 years after diagnosis) is due to poor penetration of chemotherapy into the tumor. So, the treatment requires the use of very high doses of cytotoxic chemotherapy or radical surgeries that significantly worsen the quality of life of patients. Immunotherapy on the other hand usually gives spectacular but very transitory results due to tumor resistance.

Here we propose using ShTxB functionalized nanotherapies to selectively target and destroy the neoplastic cells. As shown in our in vivo model, the treatment would consist of applying the functionalized nanoparticles locally. The ShTxB-coated nanoparticles would specifically bind to receptors on preneoplastic and malignant cells, penetrating their interior, and ultimately destroying the cancer cells upon activation by locally near-infrared LD irradiation. There are many advantages related to the topical use of these nanoparticles. Among others, they do not cause an immunoreaction, nor are prematurely eliminated by phagocytes since they are not supplied parenterally. In addition, we have shown that these nanosystems are safe by design until laser irradiation so, in case of being swallowed they can travel along the digestive tract until they are safely eliminated. This treatment may be used as an adjuvant method to enhance the effects of these standard treatments, improving the recovery and survival rates of patients while preventing local recurrences. Furthermore, the nanoparticles presented herein could also be used for the treatment of cancers in other regions of the digestive tract where GB3 has also been reported, including cancers of the esophagus, stomach, or colon.13,16 In these cases, a laser fiber could be coupled to an endoscope system to guarantee access to the relevant areas of the digestive tract. Furthermore, there is the possibility of using the ShTxB toxin fragment as a biosensor. For this, a double wavelength laser could be used. The green laser light would be used to identify the area affected by the tumor (GB3+ve) delimited by the red fluorescence of the fluorescent AuNRs and, switching to a NIR LD wavelength of 808 nm, photohyperthermia treatment will be used to kill the neoplastic cells directly, or repeatedly, by applying the particles and laser over the affected area following a “layer by layer” elimination procedure.

Conclusion

This study demonstrates that the local (topical) application of nanomaterials targeted by high-affinity natural ligands in combination with photo-hyperthermia has enormous potential as a treatment for localized neoplasms such as HNC, the sixth most common cancer worldwide. The designed nanosystem model could serve as a theranostic nanoparticle capable of detecting and eliminating neoplasms that, in their early stages, often escape detection by standard clinical methods.

Acknowledgments

We are grateful to Débora Muñoz for her technical support and the IDIVAL microscopy service. MLF acknowledges ISCIII Grants PI19/00349 and DTS19/00033, co-funded by the European Regional Development Fund, “Investing in your future”; COST action Nano2Clinic CA17140, and IDIVAL for the PREVAL16/02, INNVAL20/13 and INNVAL21/19 projects. L.M.L.M. acknowledges funding from the European Research Council (ERC AdG 787510, 4DbioSERS) and the Maria de Maeztu Units of Excellence Program from the Spanish State Research Agency (Grant No. MDM-2017-0720). RV acknowledges financial support from Spanish Ministerio de Ciencia, Innovación y Universidades (PGC2018-101464-B-I00) and HIPERNANO RED2018-102626-T). A.G. acknowledges ISCIII/FIS-FEDER Grant PI20/00880. J.G. acknowledges the predoctoral scholarship from Asociación Española Contra el Cáncer (AECC; Spain), PRDCA19003GALA. Figures 1C, 2A, 3A and 4A have been created with BioRender.com.

Disclosure

The authors report no conflicts of interest in this work.

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