Jump to ContentJump to Main Navigation
Show Summary Details
More options …


Open Access
See all formats and pricing
More options …
Volume 16, Issue 1


Cell-penetrating peptides for nanomedicine – how to choose the right peptide

Ilja Tabujew / Marco Lelle / Kalina Peneva
Published Online: 2015-05-21 | DOI: https://doi.org/10.1515/bnm-2015-0001


More than two decades ago, a group of peptides, now known as cell-penetrating peptides, sparked the hope that the ultimate carrier molecules have been found. The high expectations for these peptides, which are reflected in their bold name, led to many disappointments due to the controversial results their utilization entailed and nowadays even their effectiveness has been called into question. In this review, we discuss the uptake mechanism and application of cell penetrating peptides as mediators for organelle specific delivery of nanocarriers, pointing out the possibilities as well as strategies of their successful utilization. Additionally, we provide an overview of the conjugation techniques usually employed for the attachment of cell penetrating peptides to quantum dots, as well as silver and gold nanoparticles, and we address the various aspects that need to be considered for the successful implementation of cell penetrating peptides for organelle-specific delivery of nanoparticles into cells.

This article offers supplementary material which is provided at the end of the article.

Keywords: cell penetrating peptide; drug delivery; gold nanoparticle; nanomedicine; polymeric nanoparticle; quantum dot


  • We discuss the mechanisms of cell penetrating peptide’s uptake and briefly introduce the different types of peptides in order to present a more complete picture of the intracellular fate of the peptide-cargo conjugates.

  • We highlight the recent applications of cell penetrating peptides in the targeted delivery of quantum dots as well as gold, silver and polymeric nanoparticles into mammalian cells in the context of organelle specificity.

  • We give a short overview of the conjugation techniques usually utilized for the attachment of cell penetrating peptides to quantum dots as well as silver and gold nanoparticles.


The plasma membrane and membranes of organelles are impermeable barriers to many biologically active molecules and carrier systems. More than two decades ago, Frankel and Pabo [1] as well as Green and Loewenstein [2] simultaneously reported the first peptide, which was able to cross the aforementioned barriers. The peptides exhibiting these properties, now known as cell-penetrating peptides (CPP) [3], “Trojan peptides” or protein transduction domains (PTD), sparked hope that the ultimate carrier molecules for the transport of small molecules and nanocarriers have been found. Since then, the literature has witnessed more than 4000 publications on CPPs and our understanding of their nature as well as the mechanism of uptake has been enhanced greatly. However, the more we know about these small peptides, the more questions arise. The high expectations of CPPs, which are reflected in their bold name, led to many disappointments and even their effectiveness has been called into question [4]. Several studies have reported their limited applicability in vivo, including the work of Caron et al. [5], who demonstrated that even subcutaneous and intra-arterial injections of CPP modified green fluorescent proteins (Tat-eGFP) led to only few stained fibers in the muscle periphery or those surrounding the blood vessels. On the other hand, CPPs offer advantages over other carrier systems for the therapeutic as well as diagnostic delivery of cargo. They have been employed for the delivery of a large variety of molecules and particles ranging from small drugs and fluorophores to proteins, polymer conjugates as well as nanoparticles, which can be further divided into several classes of inorganic nanomaterials differing in their nature as well as in their function. This review will highlight the recent applications of CPPs in the targeted delivery of their most prominent examples such as quantum dots as well as gold, silver and polymeric nanoparticles into mammalian cells in the context of organelle specificity. Additionally, we will give a short overview of the conjugation techniques usually utilized for the attachment of CPPs to these nanostructures, while leaving out the modification methods of polymeric nanoparticles due to the overwhelming number of available functional groups and the entailing possibilities for conjugation chemistry, which would be beyond the scope of this review. In order to present a more complete picture of the intracellular fate of the CPP-cargo conjugates, we will also discuss the mechanisms of peptide uptake and briefly introduce the different types of CPPs.

Types of CPPs

A large number of CPPs have been isolated and designed to facilitate intracellular delivery of therapeutic molecules. In the past, cell penetrating peptides were often classified as protein derived, model peptides or designed CPPs [6], however, the categorization in cationic, hydrophobic or amphipathic CPPs is becoming more common (see Table 1) [38]. Cationic CPPs were the first to be discovered starting with the HIV-1 derived Tat-peptide, which is by far the most intensely studied CPP [1]. Peptides belonging to this class often possess short arginine-, lysine- or histidine-rich amino acid sequences, which interact electrostatically with the negatively charged phosphates and sulfates on the plasma membrane that leads to receptor-independent internalization [39, 40]. The guanidinium groups of arginine are protonated at physiological conditions, whereas the amino groups of lysine and histidine are only partially protonated, making CPPs with an oligoarginine sequence the most effective in this type of carrier-cell interaction. In addition, it has been demonstrated that cationic CPPs require at least eight positive charges for efficient cellular uptake [41]. Hydrophobic peptides, on the other hand, are distinguished due to the hydrophobicity of the incorporated amino acids and their low net charge. Amphipathic CPPs possess lipophilic, as well as hydrophilic segments, of their sequence and can be further categorized in primary amphipathic CPPs (Pep-1), secondary amphipathic α-helical CPPs (hCT18-32), β-sheet amphipathic CPPs (VT5) and proline-rich amphipathic CPPs (Bac7) [38]. In this review, we will only highlight the CPPs most often applied for the delivery of nanomedicine, however, for a detailed and comprehensive description of all existing CPPs the reader is directed to the review by Milletti [38].

Table 1

Examples for CPP-mediated transport of various cargo including the proposed uptake mechanism.

Uptake mechanism

In spite of the fact that CPPs have been employed in a wide range of applications for more than two decades and although several internalization models have been suggested (Figure 1), the exact uptake mechanism of the various CPPs still remains to be fully unveiled [42, 43]. Koppelhaus et al., for example, investigated Tat- and penetratin-mediated cellular uptake of peptide nucleic acid oligomers in five different cell lines (HeLa, SK-BR-3, IMR-90, H9 and U937) demonstrating poor or no uptake at all [44]. The authors concluded that the efficiency of the internalization largely depends on the composition of the membrane (membrane-bound components and lipids). Heparan sulfate proteoglycans (HSPGs), cell surface proteoglycans composed of a core protein and one or more heparan sulfate (HS) glycosaminoglycan (GAG) chains [45], have been recently shown to interact electrostatically with CPPs as initial binding sites, which increase the local concentration of CPP-cargo conjugates and as a consequence promote internalization [46–49]. In particular, arginine rich CPPs such as Tat, penetratin or oligoarginine, which possess a positive net charge at physiological conditions, show a high affinity towards HSPGs, one of the most highly negatively charged biopolymers [50]. Besides the HSPG-mediated cellular uptake other uptake mechanisms have also been described such as the clathrin-dependent, caveolae-mediated and the clathrin/caveolae-independent endocytosis (see Figure 1) [43]. Understanding the internalization route a CPP-cargo conjugate takes is an important step for successful organelle-specific targeting. The energy-independent route of direct translocation into the cytosol, for example, can circumvent the setbacks of vesicular trapping of cargo, as well as need of endosomal escape mechanisms, and therefore facilitates the targeting of cellular structures such as the nucleus or the mitochondria. However, depending on the employed CPP, the plasma membrane composition of the cell type, as well as on the characteristics of the cargo molecule, either endocytosis or direct translocation can be the predominant uptake mechanism [51]. The intracellular fate of their cargo can also be influenced, for example, by equipping the carrier system with sorting peptides, hence exploiting the subtle differences of vesicle membrane composition of the respective uptake mechanisms [52]. Therefore, all of these parameters need to be taken into account when choosing a CPP and it is wrong to assume that a certain CPP, which has been shown to deliver therapeutic molecules in a definite way into selected cells, would be able to do the same for other cargo or other cell lines. Table 1 and Figure 1 depict the complexity of this topic, since they also show that even systems which are similar in cargo type as well as the used CPP, can lead to different uptake mechanisms simply due to variations in shape and size of the cargo. An increase in size of the CPP-cargo conjugate, for example, diminishes the direct translocation and enhances the energy dependent endocytotic uptake [53]. Adsorptive transcytosis (AMT), a time- and energy-dependent endocytotic mechanism, enables molecules to cross the blood-brain barrier (BBB) [54]. Since AMT largely depends on electrostatic interaction between the cell-surface of the brain capillary network, which possesses a highly negative charge density, and the positive charge of the crossing molecule, cationic arginine rich CPPs can be exploited for the successful delivery of conjugated cargo molecules without affecting the biological activity [55]. However, the exact mechanism of AMT for the transport of CPP-cargo conjugates across the BBB still remains unknown, in spite of its proven efficiency [56].

Schematic representation of the various uptake mechanisms for cell penetrating peptide-modified nanoparticles illustrating the dependency of the internalization pathway on the chosen cell penetrating peptide as well as the shape, size and type of the cargo.
Figure 1:

Schematic representation of the various uptake mechanisms for cell penetrating peptide-modified nanoparticles illustrating the dependency of the internalization pathway on the chosen cell penetrating peptide as well as the shape, size and type of the cargo.

CPP mediated delivery of nanoparticles

Cell-compartment targeting with CPPs

The most promising property of CPPs is the possibility to combine targeting and transduction properties [57–59]. CPPs can influence tissue localization of a conjugated molecule by altering organ distribution and retention. In the work of Kameyama et al., for example, the CPPs REV (TRQARRNRRRRWRERQR-GC), Tat (GRKKRRQRRRPPQ-C), and ANP (Antennapedia (43–58), RQIKIWFQNRRMKWKK-GC) were conjugated to the Fab unit of an antibody (antigen binding domain) and significant changes in the distribution as well as retention in organs, such as spleen, liver, adrenal gland and kidney, were observed [60]. Targeting at subcellular level is also possible, enabling the delivery of biologically active substances into different cellular compartments such as Golgi apparatus, mitochondria or nuclei (see Table 1). Organelle-specific targeting can be achieved, for example, by utilizing signal peptides, which are a common tool used by cells for sorting and trafficking of newly translated proteins [61]. Nuclear localization sequences (NLS), which consist of roughly 10 amino acids and possess a high cationic net charge as well as inherent cell-permeation properties [62], belong to the above-mentioned class of signal peptides. Nuclear localization and transfection efficiency, important properties for gene therapy, have been repeatedly demonstrated for NLS-mediated [59, 63–65] delivery of not only polymer or phage particle encapsulated DNA [66, 67], but also of gold nanoparticles [37] and proteins [68]. Signal peptides also enabled efficient targeting of mitochondria, which are of great interest for drug delivery, as mitochondria house the protein complexes of the electron transport chain [69], generate reactive oxygen species and are therefore essential for cell proliferation [70] and intracellular signaling [71, 72]. However, the naturally abundant signal sequences for mitochondrial targeting cannot be utilized for organelle specific delivery since they are only functional in the presence of the respective full-length protein [73]. Artificial signal sequences offer a way to circumvent this setback. Zhao et al. utilized tetrapeptide sequences such as SS-02 (Dmt-D-RFK-NH2), SS-20 (Phe-D-RFK -NH2), SS-31 (D-R-Dmt-KF-NH2) in order to achieve localization of antioxidants in mitochondria as a means to arrest the progress of apoptosis by incorporating the unnatural amino acid 2,6-dimethyltyrosine (Dmt), a radical scavenger, into the sequences [34]. Horton et al. developed different peptide sequences (to-FXrFXKFXrFXK, to-FrFXKFrFXK, to-FrFKFrFK, to-FrYKFrYK with Fx=cyclohexylalanine, to=Thiazole orange and r=d-arginine) containing cationic as well as lipophilic residues for mitochondrial targeting, which were additionally shown to possess cell-penetrating properties [35]. They demonstrated that these octameric sequences with varying degrees of lipophilicity and cationic charge led to localization in either mitochondria or the nucleus and cytosol. Kelley and coworkers further described a molecular charge dependent lipophilicity threshold, which governs organelle targeting. Subcellular localization in mitochondria and the nucleus was achieved by altering the sequence of the signal peptides and by conjugating the peptides to Thiazole orange. These organelle-targeting properties of peptides, which are also able to transport cargo across plasma membranes, have been repeatedly applied for drug delivery applications. The advantage of equipping a cargo molecule with both traits in only one step has also been capitalized upon in a variety of recent studies on nanoparticles, which will be introduced in the next section.

Delivery of nanoparticles using CPPs

Quantum dots

Fluorescent markers are a useful tool for studying living cells due to their ability to illuminate intracellular or exogenous molecules and are often applied to observe and investigate various dynamic cellular processes [74]. Quantum dots (QDs) are nanocrystals with a core diameter of 1–6 nm. They can be comprised of varying elements (groups II to IV or III to V), but CdSe and CdTe are the most commonly used in life science [75]. The use of non-biodegradable heavy metals for clinical applications, however, requires careful consideration of their biodistribution and long term toxicity [76]. It is therefore important to ensure rapid renal clearance of QDs by utilizing to a small final hydrodynamic radius (<5.5 nm) and formulations with completely nontoxic as well as biodegradable coating-components [77, 78]. These coatings are also usually used to improve the solubility in aqueous media and as a means to equip quantum dots with functional groups, which in turn are necessary for the subsequent conjugation of bioactive molecules (Figure 3A). QDs are often depicted as excellent candidates for fluorescent labeling especially for prolonged observations, since they possess not only resistance to photobleaching, high quantum yields, as well as tunable photoexcitation [79], but also sharply defined emission peaks [80]. However, they are not able to cross plasma membranes unaided, since, as a result of common synthetic procedures, QDs are water-insoluble, which makes the utilization of either direct injection into cells or the modification of their surface a necessity [81, 82]. The approach of using of positively as well as negatively charged coatings for improved water solubility can be expanded by the conjugation of bioactive molecules, such as CPPs, in order to influence the uptake mechanism and intracellular targeting [83, 84]. Xue et al., for instance, conjugated Tat peptide to thiol capped CdTe QDs (2–4 nm in diameter) and compared their effectiveness in intracellular delivery to unmodified CdTe QDs in human hepatocellular carcinoma (QGY) cells and human breast cancer (MCF7) cells by means of confocal laser scanning microscopy. The authors were able to demonstrate that the conjugation of Tat enhanced intracellular delivery in both cell lines [85]. The same holds true for the PEG-encapsulated CdSe-ZnS QDs, which were functionalized with covalently bound Tat in order to achieve efficient uptake into mesenchymal stem cells [86]. In a study by Liu et al. CPPs did not need to be covalently associated to QDs to achieve efficient cellular internalization. This non-covalent attachment of histidine- and arginine-rich peptides to carboxylated QDs allowed for direct membrane translocation and diminished the setback of endosomal, as well as lysosomal trapping [87]. Equipping QDs with cysteine-terminated NLS peptides, such as the adenovirus-derived CGGFSTSLRARKA, the SV40 large T antigen-derived CGGGPKKKRKVGG or the HIV-1 Tat protein-derived CGGRKKRRQRRRAP by means of the heterobifunctional linker (Succinimidyl-4-[N-maleimidomethyl]cyclohexane-1-carboxylate) led to efficient cellular internalization. This modification also allowed active targeting of the nucleus in spite of the increased size of the particles (14.1–18 nm in diameter) [36]. We should mention that the cellular uptake can be influenced not only by the conjugation of CPPs, but also by the number of QD-associated CPPs and the cell-type, which has been confirmed by Delehanty et al. [88] The functionalization of QDs with CPPs can facilitate their transport across the plasma membrane, and thus enable these particles to cross the blood-brain barrier (BBB). Tat-modified QDs, for example, were successfully used by Santra et al. to fluorescently label brain tissue of rodents (SD adult rats, Sprague-Dawley rats) [89].

Silver and gold nanoparticles

Silver nanoparticles possess a broad spectrum of valuable optical, electrical, thermal and antibacterial properties. A great wealth of information regarding their biocompatibility has been collected, as silver has been applied for medical purposes since the Middle Ages, and silver nanoparticles are still being applied as a component for antimicrobial coatings of textiles, wound dressings and other biomedical devices. The cytotoxicity of silver nanoparticles has been reported to result from their size and the solvatization of the particles in a codependent manner [90]. Liu et al. were able to further enhance the biocidal effect of silver nanoparticles towards bacteria by coating the particles with CPPs such as Tat by the DMF reduction method, which indicates that the surface modification is of greater importance for the biocidal properties than the size and shape of the nanoparticles [91]. Liu et al. used a modification method, which utilizes the thiol functionality of cysteine terminated peptides, in order to equip silver nanoparticles (8 nm in diameter) with the Tat peptide and provided a proof of concept for the size-exclusion mechanism of multidrug-resistant (MDR) tumor cells. These modified nanoparticles demonstrated not only efficient cell-uptake, but also showed antitumor activity in MDR, as well as non-resistant tumor cells, while exhibiting reduced adverse toxicity in vivo [14].

Gold nanoparticles have unique optical and electronic properties, which can also be tuned by size, shape and surface chemistry, making them highly useful for high technology applications. However, these non-biodegradable but biocompatible particles are also exceptional therapeutic tools in biological and medical applications, such as the delivery of drug molecules and bioactive agents, due to their large surface area and their ability to selectively incorporate recognition molecules such as peptides or proteins [92, 93]. The advantageous properties of gold nanoparticles lead to numerous studies investigating their toxicity and metabolization in various model organisms. The findings indicated low toxicity and efficient renal clearance, if the hydrodynamic radius of the said particles did not exceed 5–6 nm [94, 95]. The toxicity of gold nanoparticles also largely depends on the surface modifications [96]. Therefore, similarly to their silver counterparts, gold nanoparticles require not only fine-tuned radii but also functionalization with engineered coating, which promote targeting and hydrophilicity, in order to realize their full potential in drug delivery applications [52]. The conjugation of CPPs for improved internalization and specific organelle targeting is a prime example for further improvement of their innate properties, as unmodified nanoparticles cannot cross the plasma membrane unaided prohibiting targeted localization in the nuclei or other organelles [97]. NLS peptides have been largely utilized to achieve this aim. Feldheim and colleagues described the delivery of bovine serum albumin (BSA) coated gold nanoparticles into the nuclei of HepG2 cells by means of conjugating these particles with a diameter of 20 nm to NLS of different viruses [37]. The attachment of Tat is another method to achieve efficient cellular internalization and nuclear localization of nanomedicine. This approach has been used by de la Fuente et al., who conjugated Tat to tiopronin protected gold nanoparticles of adequate size (2.8 nm in diameter) to pass through the nuclear pores of primary human fibroblast cells (hTERT-BJ1) [15]. In this context it is important to mention that Krpetic et al. demonstrated Tat-modified gold nanoparticles (14 nm in diameter) to possess not only enhanced internalization into HeLa cells, but also a peculiar distribution pattern: The aforementioned modified nanoparticles were initially found in the cytosol, the nucleus and mitochondria, appearing to cross intracellular membranes freely. Later, they were densely packed within vesicles, from which they were subsequently released by membrane rupture or direct transfer across the membrane [98]. Therefore, the cargo was found in various cell compartments indiscriminately making organelle specific targeting impossible. Avoiding unselective cytotoxicity originating from the cargo, however, is a necessity for drug delivery purposes. Dekiwadia et al. achieved the desired specificity by equipping gold nanoparticles with a combination of CPPs and lysosomal sorting peptides for the treatment of storage diseases by delivering replacement enzymes into lysosomes [52]. Combining ionic and covalent formulation approaches, Conde et al. functionalized gold nanoparticles with a diameter of 14 nm with PEG chains, arginine-glycine-aspartic (RGD) targeting peptide as well as Tat. The resulting particles showed excellent biocompatibility, low cytotoxicity and good chemical stability when tested in Hela cells, freshwater polyps (Hydra vulgaris) and mice (C57BL/6j) [97].

In a recent study Oh et al. investigated the internalization and intracellular fate of Tat functionalized gold nanoparticles with varying diameters ranging from 2.4 to 89 nm. The authors we able to demonstrate that although the conjugated CPPs were largely responsible for the cellular uptake, the final cellular target was influenced by the diameter of the nanoparticles. Small nanoparticles (2.4 nm) localized preferably in the nuclei, intermediate particles (5.5–8.2 nm) were partially found in the cytosol and particles with a diameter exceeding 16 nm were not internalized in spite of the functionalization with CPPs [99]. Ryan et al. studied BSA coated gold nanoparticles with a diameter of 15 nm, which were equipped with modified SV40 large T antigen-derived peptides (rhodamine-Cys-Gly-Gly-Gly-Pro-Lys-Lys-Lys-Arg-Lys-Val-Gly-Gly-OH) and they were able to demonstrate that intracellular entry depends not only on the size but also on the number of CPPs positioned on the particle’s surface [100]. We should also note here that additional factors such as the cell type, nature and origin (e.g., adenovirus, SV40, or HIV-1) of the CPP, incubation time and the temperature during the experiment, which were not discussed in this review, can also strongly influence the efficiency of internalization of a CPP-nanomedicine conjugate [101].

Polymeric nanoparticles

Polymeric nanoparticles can be defined as structures with a diameter of <1 μm and are prepared from either natural or synthetic polymers. Natural polymers, such as polysaccharides, are suited for drug delivery applications due to their low toxicity and bioavailability [102]. However, they exhibit batch-to-batch differences and vary in purity making biocompatible and biodegradable synthetic polymers, such as poly(lactic acid) (PLA), poly(glycolic acid) (PGA) or their copolymers [poly(lactide-co-glycolide) (PLGA)] the preferred choice [103]. Due to the large variety of applicable polymers and the resulting possibilities of design a wide range of cargo such as hydrophilic and hydrophobic drugs, proteins as well as vaccines can be delivered to diverse areas of the body for sustained periods of time. This performance, however, is only possible due to the numerous synthesis protocols and surface modification strategies [103]. The conjugation of CPPs improves the utility of polymeric nanocarriers, since these particles can neither cross the BBB unaided nor are they able to penetrate plasma membranes efficiently. Various examples for the successful utilization of CPPs for the enhanced delivery of polymeric nanoparticles exist, such as the Penetratin-functionalized PLA-PEG nanoparticles, which demonstrated successful delivery into brain cells. In comparison to conjugates with arginine-rich CPPs, this conjugate was also shown to possess reduced non-target tissue accumulation [23]. Jiang et al. equipped polyethylenimine-β-cyclodextrin nanoparticles (PEI600-CyD) with oligoarginine (R8) as well as folic acid targeting ligands in order to improve the efficiency of gene delivery into rat glioma cells (C6 cells) [7]. Another example for the successful application of CPPs for polymeric nanoparticle delivery is the work of Jabbari et al., who exploited the hydrophilic properties of the V6K2 peptide (VVVVVVKK), which was conjugated to low-molecular-weight polylactide, in order to facilitate encapsulation of doxorubicin and paclitaxel as well as cellular uptake by 4T1 murine breast carcinoma cells [104]. Similarly to the other introduced nanosized materials, which have been described in this review, not only the surface modification but also the shape and size of polymeric nanoparticles can impact the cellular internalization. Zhang et al. investigated Tat modified spherical micelles (11 nm diameter) as well as short (20 nm diameter, 180 nm length) and long (30 nm diameter, 970 nm length) cylindrical micelles, which consisted of poly(acrylic acid)-polystyrol block copolymers, in order to underpin this statement [105]. They were able to demonstrate that the internalization efficiency of spherical micelles into cells is dependent on the CPP loading. The Tat-functionalization of short as well as long cylindrical micelles, on the other hand, did not improve the uptake efficiency. This effect was observed for low as well as high peptide loading and can only be attributed to the differences in size and shape.

Conjugation approaches

The advantages of CPP modified nanoparticles in regard to biological compatibility, targeting and cellular uptake of different cargo have been pointed out in previous sections. However, since the amount of bound cell penetrating peptides can affect the internalization properties and cellular distribution of the cargo, making conjugation efficiency an important factor in carrier design, it is also important to give insight into the existing functionalization methods of nanoparticles.

The surface modification of gold nanoparticles is largely based on the work of Whitesides and Nuzzo [106, 107], who investigated the formation of self-assembled monolayers of molecules on planar gold. Bioactive molecules, such as CPPs, can be conjugated to the surface of gold nanoparticles by means of various passivating agents and linkers. The multifunctional passivating agents possess conjugation chemistry-facilitating functional groups as well as anchoring groups, such as thiolates [108], dithiolates [109], dithiocarbamates [110], amines [92], phosphines [111], carboxylates [92], and isothiocyanates [92], which enable the said molecules to coat the surface of gold nanoparticles. The choice of the anchor functionality depends on the desired stability of the established bond between the gold nanoparticle and conjugated molecule. The weak interaction between amine or carboxylate anchor groups and the gold surface, for example, leads to continuous release of the cargo, which is undeniably advantageous for gold nanoparticle mediated drug delivery [112]. Thiol-based anchors, on the other hand, ensure stability and even cysteine terminated peptides were successfully used in order to coat gold nanoparticles [98, 113]. Thiolates, which do not suffer from oxidative desorption in the same manner as dithiolates, remain adsorbed to the gold surface for 35 days at physiological conditions and are therefore most commonly applied for the attachment of CPPs [114]. While the hydrophobic entrapment and charge-pairing (Figure 2B) play only a minor role for the attachment of CPPs to gold nanoparticles, classic coupling reagents, such as 1-Ethyl-3-(3-dimethylaminopropyl)carbodiimide (EDC) or N-Hydroxysuccinimide (NHS) esters, on the other hand, are a useful tool in order to establish the desired stable chemical bond [15, 97, 100]. The same can be achieved by means of Michael addition or click-chemistry (Figure 2A). Peptides are commonly conjugated to gold nanoparticles in this fashion and a variety of commercially available heterobifunctional polymers, as well as linkers with terminal maleimides, N-hydroxysuccinimide activated carboxylic groups or azide functional groups are available for the functionalization of gold nanoparticles with CPPs [115–117]. In some cases it is also possible to utilize bovine serum albumin (BSA) as the reducing agent in order to synthesize BSA-coated gold nanoparticles, which can be used as a scaffold for the attachment of CPPs [37, 118].

Functionalization of gold nanoparticles by (A) covalent coupling of bioactive molecules using carbodiimide, maleimide or click chemistry, (B) electrostatic adsorption and (C) direct functionalization of ligand-free gold nano particles.
Figure 2:

Functionalization of gold nanoparticles by (A) covalent coupling of bioactive molecules using carbodiimide, maleimide or click chemistry, (B) electrostatic adsorption and (C) direct functionalization of ligand-free gold nano particles.

Quantum dots (QD) possess different physicochemical properties than the noble metal nanoparticles and therefore require an alternative surface conjugation approach. Several methods have been developed for the design of water-soluble QDs by using polymers, thiols (Figure 3B) and silanization (Figure 3C) [119, 120]. Such coatings are not only required to improve the water solubility but also to equip the QD with functional groups, which in turn are needed for further modification and conjugation chemistry (Figure 3B). Tiopronin coated CdS QDs, for example, were functionalized with Tat peptide by using a ligand exchange method (Figure 3A) in order to achieve nuclear targeting in hTERT-BJ1 human fibroblasts [13]. Similar coating approaches have been used by Wei et al., by functionalizing CdSe-ZnS QDs with Tat for cell staining. However, the authors utilized not only the ligand exchange method but also the covalent conjugation of the cell-penetrating peptide to silan or polyacrylate coated QDs. The different coating approaches that were employed led to Tat-functionalized QDs with different sizes (6–25 nm in diameter) and surface charge (+8 to +35 mV), which in turn influenced the cellular uptake and subcellular targeting specificity. The particles with a diameter of 6 nm and a surface charge of +8 mV were taken up poorly but mainly showed perinuclear localization. Increasing their size and surface charge improved cellular uptake while diminishing their targeting specificity. Wei et al. were also able to demonstrate that nanoparticles with a diameter exceeding 13 nm were primarily taken up by endosomal pathways [121]. Another efficient conjugation technique was employed by Lagerholm et al., who utilized biotinylated oligoarginine in order to equip commercially available streptavidin-coated QDs with cell-penetrating properties for multicolour staining of mammalian cells [embryonic mouse fibroblasts (Swiss 3T3), human endothelial cells (HeLa), and human osteoblast-like cells (MG63)]. These modified QDs, however, were reported to be internalized solely by endocytosis [8]. The interaction of biotin and streptavidin was also exploited by Mok et al. for the preparation of PEGylated QDs, which could be specifically dePEGylated in the presence of the matrix metalloprotease-2 enzyme for targeted cellular uptake [26]. This effect was achieved due to the immobilization of biotin-PEG conjugates onto streptavidin-coated QDs by utilizing peptide-linkers, which were a substrate for the peptidase. In addition, the biotinylated CPP Hph-1 (YARVRRRGPRR) was immobilized onto the surface of the PEGylated QD as well, in order to enhance the cellular uptake after dePEGylation. The introduced variety of modification methods for quantum dots and noble metal nanoparticles provide a basic set of necessary possibilities to optimize the conjugation efficiency of CPPs onto nanoparticles, which is crucial for customizing not only cellular distribution, but also uptake efficiency.

Functionalization of quantum dots (A) Composition of a functionalized QD (B) Partial and complete ligand exchange (C) Silanization.
Figure 3:

Functionalization of quantum dots (A) Composition of a functionalized QD (B) Partial and complete ligand exchange (C) Silanization.


In this review we discussed the uptake mechanisms and the viability of CPPs as mediators for organelle specific delivery of nanoparticles, pointing out the possibilities and strategies of their successful utilization. Such functionalization of carrier-systems with CPPs, however, has become a controversial topic. Ever since their discovery, CPPs have been investigated as versatile components for drug delivery systems and although a large number of studies claim nearly unrestricted cellular internalization, researchers face the hurdles of CPP-mediated cellular access, which are not only restricted to metabolic degradation. The properties of the cargo as well as the varying composition of the membrane of cell lines and cellular differentiation can significantly influence the efficiency of cellular uptake. When considering these findings, it is unrealistic to expect that all CPP-conjugated cargo can be delivered across every type of membrane just because of their bold name. Here, we have shown the various aspects that need to be considered for the successful implementation of CPPs for organelle-specific delivery of nanoparticles into cells. We believe that a methodical approach to their study as well as guidelines for their selection, which consider all aspects of CPP-mediated delivery, need to be introduced in the future. In spite of the mentioned obstacles, the wealth of inspiring ideas and the long list of successful applications of CPPs has given rise to an ever-growing field of studies with more than 1150 scientific publications just in 2014, which corresponds to a rise of 32% in comparison to the number registered in 2009 and the trend is still rising. Therefore, the modification of cargo with CPPs will remain an effective strategy to improve the efficiency of the transport across plasma membranes, especially considering their organelle-targeting properties.


  • 1.

    Frankel AD, Pabo CO. Cellular uptake of the tat protein from human immunodeficiency virus. Cell 1988;55:1189–93.CrossrefGoogle Scholar

  • 2.

    Green M, Loewenstein PM. Autonomous functional domains of chemically synthesized human immunodeficiency virus tat trans-activator protein. Cell 1988;55:1179–88.CrossrefGoogle Scholar

  • 3.

    Lindgren M, Hallbrink M, Prochiantz A, Langel U. Cell-penetrating peptides. Trends Pharmacol Sci 2000;21:99–103.CrossrefGoogle Scholar

  • 4.

    Howl J, Nicholl ID, Jones S. The many futures for cell-penetrating peptides: how soon is now? Biochem Soc Trans 2007;35:767–9.CrossrefGoogle Scholar

  • 5.

    Caron NJ, Torrente Y, Camirand G, Bujold M, Chapdelaine P, Leriche K, et al. Intracellular delivery of a tat-eGFP fusion protein into muscle cells. Mol Ther 2001;3:310–8.CrossrefGoogle Scholar

  • 6.

    Eiriksdottir E, Myrberg H, Hansen M, Langel U. Cellular uptake of cell-penetrating peptides. Drug Des Rev-Online 2004;1:161–73.Google Scholar

  • 7.

    Jiang Q-Y, Lai L-H, Shen J, Wang Q-Q, Xu F-J, Tang G-P. Gene delivery to tumor cells by cationic polymeric nanovectors coupled to folic acid and the cell-penetrating peptide octaarginine. Biomaterials 2011;32:7253–62.CrossrefGoogle Scholar

  • 8.

    Lagerholm BC, Wang M, Ernst LA, Ly DH, Liu H, Bruchez MP, et al. Multicolor coding of cells with cationic peptide coated quantum dots. Nano Lett 2004;4:2019–22.CrossrefGoogle Scholar

  • 9.

    Nakase I, Niwa M, Takeuchi T, Sonomura K, Kawabata N, Koike Y, et al. Cellular uptake of arginine-rich peptides: roles for macropinocytosis and actin rearrangement. Mol Ther 2004;10:1011–22.CrossrefGoogle Scholar

  • 10.

    Khalil IA, Kogure K, Futaki S, Harashima H. High density of octaarginine stimulates macropinocytosis leading to efficient intracellular trafficking for gene expression. J Biol Chem 2006;281:3544–51.Google Scholar

  • 11.

    Iwasa A, Akita H, Khalil I, Kogure K, Futaki S, Harashima H. Cellular uptake and subsequent intracellular trafficking of R8-liposomes introduced at low temperature. Biochim Biophys Acta, Biomembr 2006;1758:713–20.Google Scholar

  • 12.

    Ruan G, Agrawal A, Marcus AI, Nie S. Imaging and tracking of tat peptide-conjugated quantum dots in living cells: new insights into nanoparticle uptake, intracellular transport, and vesicle shedding. J Am Chem Soc 2007;129:14759–66.Google Scholar

  • 13.

    de la Fuente JM, Fandel M, Berry CC, Riehle M, Cronin L, Aitchison G, et al. Quantum dots protected with tiopronin: a new fluorescence system for cell-biology studies. ChemBioChem 2005;6:989–91.CrossrefGoogle Scholar

  • 14.

    Liu J, Zhao Y, Guo Q, Wang Z, Wang H, Yang Y, et al. TAT-modified nanosilver for combating multidrug-resistant cancer. Biomaterials 2012;33:6155–61.CrossrefGoogle Scholar

  • 15.

    De la Fuente JM, Berry CC. Tat peptide as an efficient molecule to translocate gold nanoparticles into the cell nucleus. Bioconjugate Chem. 2005;16:1176–80.CrossrefGoogle Scholar

  • 16.

    Yuan H, Fales AM, Vo-Dinh T. TAT peptide-functionalized gold nanostars: enhanced intracellular delivery and efficient NIR photothermal therapy using ultralow irradiance. J Am Chem Soc 2012;134:11358–61.Google Scholar

  • 17.

    Marty C, Meylan C, Schott H, Ballmer-Hofer K, Schwendener RA. Enhanced heparan sulfate proteoglycan-mediated uptake of cell-penetrating peptide-modified liposomes. Cell Mol Life Sci 2004;61:1785–94.Google Scholar

  • 18.

    Nair BG, Fukuda T, Mizuki T, Hanajiri T, Maekawa T. Intracellular trafficking of superparamagnetic iron oxide nanoparticles conjugated with TAT peptide: 3-dimensional electron tomography analysis. Biochem Biophys Res Commun 2012;421:763–7.Google Scholar

  • 19.

    Fretz MM, Storm G. TAT-peptide modified liposomes: preparation, characterization, and cellular interaction. Methods Mol Biol 2010;605:349–59.Google Scholar

  • 20.

    Fretz MM, Koning GA, Mastrobattista E, Jiskoot W, Storm G. OVCAR-3 cells internalize TAT-peptide modified liposomes by endocytosis. Biochim Biophys Acta, Biomembr 2004;1665:48–56.Google Scholar

  • 21.

    Balayssac S, Burlina F, Convert O, Bolbach G, Chassaing G, Lequin O. Comparison of penetratin and other homeodomain-derived cell-penetrating peptides: interaction in a membrane-mimicking environment and cellular uptake efficiency. Biochemistry 2006;45:1408–20.CrossrefGoogle Scholar

  • 22.

    Amand HL, Fant K, Norden B, Esbjorner EK. Stimulated endocytosis in penetratin uptake: effect of arginine and lysine. Biochem Biophys Res Commun 2008;371:621–5.Google Scholar

  • 23.

    Xia H, Gao X, Gu G, Liu Z, Hu Q, Tu Y, et al. Penetratin-functionalized PEG-PLA nanoparticles for brain drug delivery. Int J Pharm 2012;436:840–50.Google Scholar

  • 24.

    De Coupade C, Fittipaldi A, Chagnas V, Michel M, Carlier S, Tasciotti E, et al. Novel human-derived cell-penetrating peptides for specific subcellular delivery of therapeutic biomolecules. Biochem J 2005;390:407–18.Google Scholar

  • 25.

    Rádis-Baptista G, de la Torre BG, Andreu D. Insights into the uptake mechanism of NrTP, a cell-penetrating peptide preferentially targeting the nucleolus of tumour cells. Chem Biol Drug Des 2012;79:907–15.CrossrefGoogle Scholar

  • 26.

    Mok H, Bae KH, Ahn C-H, Park TG. PEGylated and MMP-2 Specifically DePEGylated quantum dots: Comparative evaluation of cellular uptake. Langmuir 2009;25:1645–50.CrossrefGoogle Scholar

  • 27.

    Lin Y-Z, Yao S, Veach RA, Torgerson TR, Hawiger J. Inhibition of nuclear translocation of transcription factor NF-B by a synthetic peptide containing a cell membrane-permeable motif and nuclear localization sequence. J Biol Chem 1995;270:14255–8.Google Scholar

  • 28.

    Rhee M, Davis P. Mechanism of uptake of C105Y, a novel cell-penetrating peptide. J Biol Chem 2006;281:1233–40.Google Scholar

  • 29.

    Oehlke J, Scheller A, Wiesner B, Krause E, Beyermann M, Klauschenz E, et al. Cellular uptake of an α-helical amphipathic model peptide with the potential to deliver polar compounds into the cell interior non-endocytically. Biochim Biophys Acta, Biomembr 1998;1414:127–39.Google Scholar

  • 30.

    Crombez L, Aldrian-Herrada G, Konate K, Nguyen QN, McMaster GK, Brasseur R, et al. A new potent secondary amphipathic cell–penetrating peptide for siRNA delivery Into mammalian cells. Mol Ther 2009;17:95–103.CrossrefGoogle Scholar

  • 31.

    Elmquist A, Lindgren M, Bartfai T, Langel U. VE-cadherin-derived cell-penetrating peptide, pVEC, with carrier functions. Exp Cell Res 2001;269:237–44.Google Scholar

  • 32.

    Pooga M, Hallbrink M, Zorko M, Langel U. Cell penetration by transportan. FASEB J 1998;12:67–77.Google Scholar

  • 33.

    Johansson HJ, El-Andaloussi S, Holm T, Maee M, Jaenes J, Maimets T, et al. Characterization of a novel cytotoxic cell-penetrating peptide derived from p14ARF protein. Mol Ther 2008;16:115–23.CrossrefGoogle Scholar

  • 34.

    Zhao K, Zhao G-M, Wu D, Soong Y, Birk AV, Schiller PW, et al. Cell-permeable peptide antioxidants targeted to inner mitochondrial membrane inhibit mitochondrial swelling, oxidative cell death, and reperfusion injury. J Biol Chem 2004;279:34682–90.Google Scholar

  • 35.

    Horton KL, Stewart KM, Fonseca SB, Guo Q, Kelley SO. Mitochondria-penetrating peptides. Chem Biol 2008;15: 375–82.CrossrefGoogle Scholar

  • 36.

    Kuo C-W, Chueh D-Y, Singh N, Chien F-C, Chen P. Targeted nuclear delivery using peptide-coated quantum dots. Bioconjugate Chem 2011;22:1073–80.CrossrefGoogle Scholar

  • 37.

    Tkachenko AG, Xie H, Coleman D, Glomm W, Ryan J, Anderson MF, et al. Multifunctional gold nanoparticle-peptide complexes for nuclear targeting. J Am Chem Soc 2003;125:4700–1.CrossrefGoogle Scholar

  • 38.

    Milletti F. Cell-penetrating peptides: classes, origin, and current landscape. Drug Discov Today 2012;17:850–60.CrossrefGoogle Scholar

  • 39.

    Bolhassani A. Potential efficacy of cell-penetrating peptides for nucleic acid and drug delivery in canc. Biochim Biophys Acta Rev Cancer 2011;1816:232–46.Google Scholar

  • 40.

    Koren E, Torchilin VP. Cell-penetrating peptides: breaking through to the other side. Trends Mol Med 2012;18:385–93.CrossrefGoogle Scholar

  • 41.

    Futaki S, Suzuki T, Ohashi W, Yagami T, Tanaka S, Ueda K, et al. An abundant source of membrane-permeable peptides having potential as carriers for intracellular protein delivery. J Biol Chem 2001;276:5836–40.Google Scholar

  • 42.

    Khalil IA, Kogure K, Futaki S, Harashima H. Octaarginine-modified liposomes: enhanced cellular uptake and controlled intracellular trafficking. Int J Pharm 2008;354:39–48.Google Scholar

  • 43.

    Trabulo S, Cardoso AL, Mano M, Pedroso de Lima MC. Cell-penetrating peptides–mechanisms of cellular uptake and generation of delivery systems. Pharmaceuticals 2010;3:961–93.CrossrefGoogle Scholar

  • 44.

    Koppelhus U, Awasthi SK, Zachar V, Holst HU, Ebbesen P, Nielsen PE. Cell-dependent differential cellular uptake of PNA, peptides, and PNA-peptide conjugates. Antisense Nucleic Acid Drug Dev 2002;12:51–63.Google Scholar

  • 45.

    Bishop JR, Schuksz M, Esko JD. Heparan sulphate proteoglycans fine-tune mammalian physiology. Nature 2007;446:1030–7.Google Scholar

  • 46.

    Nakase I, Takeuchi T, Tanaka G, Futaki S. Methodological and cellular aspects that govern the internalization mechanisms of arginine-rich cell-penetrating peptides. Adv Drug Deliv Rev 2008;60:598–607.CrossrefGoogle Scholar

  • 47.

    Poon GM, Gariepy J. Cell-surface proteoglycans as molecular portals for cationic peptide and polymer entry into cells. Biochem Soc Trans 2007;35:788–93.CrossrefGoogle Scholar

  • 48.

    Ziegler A, Seelig J. Binding and clustering of glycosaminoglycans: a common property of mono- and multivalent cell-penetrating compounds. Biophys J 2008;94:2142–9.CrossrefGoogle Scholar

  • 49.

    Naik RJ, Chatterjee A, Ganguli M. Different roles of cell surface and exogenous glycosaminoglycans in controlling gene delivery by arginine-rich peptides with varied distribution of arginines. Biochim Biophys Acta, Biomembr 2013;1828:1484–93.Google Scholar

  • 50.

    Aamand HL, Rydberg HA, Fornander LH, Lincoln P, Norden B, Esbjoerner EK. Cell surface binding and uptake of arginine- and lysine-rich penetratin peptides in absence and presence of proteoglycans. Biochim Biophys Acta, Biomembr 2012;1818:2669–78.Google Scholar

  • 51.

    Maiolo JR, Ferrer M, Ottinger EA. Effects of cargo molecules on the cellular uptake of arginine-rich cell-penetrating peptides. Biochim Biophys Acta, Biomembr 2005;1712:161–72.Google Scholar

  • 52.

    Dekiwadia CD, Lawrie AC, Fecondo JV. Peptide-mediated cell penetration and targeted delivery of gold nanoparticles into lysosomes. J Pept Sci 2012;18:527–34.CrossrefGoogle Scholar

  • 53.

    Ma D-X, Shi N-Q, Qi X-R. Distinct transduction modes of arginine-rich cell-penetrating peptides for cargo delivery into tumor cells. Int J Pharm 2011;419:200–8.Google Scholar

  • 54.

    Gabathuler R. Approaches to transport therapeutic drugs across the blood–brain barrier to treat brain diseases. Neurobiol Dis 2010;37:48–57.CrossrefGoogle Scholar

  • 55.

    Schwarze SR, Ho A, Vocero-Akbani A, Dowdy SF. Science 1999;285:1569–72.Google Scholar

  • 56.

    Herve F, Ghinea N, Scherrmann J-M. CNS delivery via adsorptive transcytosis. AAPS J 2008;10:455–72.CrossrefGoogle Scholar

  • 57.

    Veldhoen S, Laufer SD, Trampe A, Restle T. Cellular delivery of small interfering RNA by a non-covalently attached cell-penetrating peptide: quantitative analysis of uptake and biological effect. Nucleic Acids Res 2006;34:6561–73.CrossrefGoogle Scholar

  • 58.

    Zelphati O, Uyechi LS, Barron LG, Szoka FC Jr. Effect of serum components on the physico-chemical properties of cationic lipid/oligonucleotide complexes and on their interactions with cells. Biochim Biophys Acta, Lipid Lipid Met 1998;1390:119–33.Google Scholar

  • 59.

    Cartier R, Reszka R. Utilization of synthetic peptides containing nuclear localization signals for nonviral gene transfer systems. Gene Ther 2002;9:157–67.CrossrefGoogle Scholar

  • 60.

    Kameyama S, Horie M, Kikuchi T, Omura T, Takeuchi T, Nakase I, et al. Effects of cell-permeating peptide binding on the distribution of 125I-labeled fab fragment in rats. Bioconjugate Chem 2006;17:597–602.Google Scholar

  • 61.

    Davis JR, Kakar M, Lim CS. Utilization of synthetic peptides containing nuclear localization signals for nonviral gene transfer systems. Pharm Res 2007;24:17–27.Google Scholar

  • 62.

    Morris MC, Chaloin L, Mery J, Heitz F, Divita G. A novel potent strategy for gene delivery using a single peptide vector as a carrier. Nucleic Acids Res 1999;27:3510–7.CrossrefGoogle Scholar

  • 63.

    Goldfarb DS, Gariepy J, Schoolnik G, Kornberg RD. Synthetic peptides as nuclear localization signals. Nature 1986;322:641–4.Google Scholar

  • 64.

    Ludtke JJ, Zhang G, Sebestyen MG, Wolff JA. A nuclear localization signal can enhance both the nuclear transport and expression of 1 kb DNA. J Cell Sci 1999;112:2033–41.Google Scholar

  • 65.

    Zanta MA, Belguise-Valladier P, Behr J-P. Gene delivery: a single nuclear localization signal peptide is sufficient to carry DNA to the cell nucleus. Proc Natl Acad Sci USA 1999;96:91–6.CrossrefGoogle Scholar

  • 66.

    Jeon O, Lim H-W, Lee M, Song SJ, Kim B-S. Poly(l-lactide-co-glycolide) nanospheres conjugated with a nuclear localization signal for delivery of plasmid DNA. J Drug Targeting 2007;15:190–8.CrossrefGoogle Scholar

  • 67.

    Eguchi A, Furusawa H, Yamamoto A, Akuta T, Hasegawa M, Okahata Y, et al. Optimization of nuclear localization signal for nuclear transport of DNA-encapsulating particles. J Controlled Release 2005;104:507–19.Google Scholar

  • 68.

    Wagstaff KM, Glover DJ, Tremethick DJ, Jans DA. Histone-mediated transduction as an efficient means for gene delivery. Mol Ther 2007;15:721–31.Google Scholar

  • 69.

    McBride HM, Neuspiel M, Wasiak S. Mitochondria: more than just a powerhouse. Curr Biol 2006;16:R551–60.CrossrefGoogle Scholar

  • 70.

    Fruehauf JP, Meyskens FL Jr. Reactive oxygen species: a breath of life or death? Clin Cancer Res 2007;13:789–94.CrossrefGoogle Scholar

  • 71.

    Bayir H, Fadeel B, Palladino MJ, Witasp E, Kurnikov IV, Tyurina YY, et al. Apoptotic interactions of cytochrome c: redox flirting with anionic phospholipids within and outside of mitochondria. Biochim Biophys Acta, Bioenerg 2006;1757:648–59.Google Scholar

  • 72.

    Kagan VE, Bayir HA, Belikova NA, Kapralov O, Tyurina YY, Tyurin VA, et al. Cytochrome c/cardiolipin relations in mitochondria: a kiss of death. Free Radical Biol Med 2009;46:1439–53.Google Scholar

  • 73.

    Farkhani SM, Valizadeh A, Karami H, Mohammadi S, Sohrabi N, Badrzadeh F. Cell penetrating peptides: efficient vectors for delivery of nanoparticles, nanocarriers, therapeutic and diagnostic molecules. Peptides 2014;57:78–94.CrossrefGoogle Scholar

  • 74.

    Stephens DJ, Allan VJ. Light microscopy techniques for live cell imaging. Science 2003;300:82–6.Google Scholar

  • 75.

    Resch-Genger U, Grabolle M, Cavaliere-Jaricot S, Nitschke R, Nann T. Quantum dots versus organic dyes as fluorescent labels. Nat Methods 2008;5:763–75.CrossrefGoogle Scholar

  • 76.

    Tsoi KM, Dai Q, Alman BA, Chan WC. Are quantum dots toxic? Exploring the discrepancy between cell culture and animal studies. Acc Chem Res 2013;46:662–71.CrossrefGoogle Scholar

  • 77.

    Choi HS, Liu W, Misra P, Tanaka E, Zimmer JP, Ipe BI, et al. Renal clearance of quantum dots. Nat Biotechnol 2007;25:1165–70.CrossrefGoogle Scholar

  • 78.

    Vengala P, Dasari A, Yeruva N. Quantum dots for drug delivery and therapy. Int J Pharm Technol 2012;4:2055–74.Google Scholar

  • 79.

    Huang X, Weng J, Sang F, Song X, Cao C, Ren J. Characterization of quantum dot bioconjugates by capillary electrophoresis with laser-induced fluorescent detection. J Chromatogr A 2006;1113:251–4.Google Scholar

  • 80.

    Delehanty JB, Mattoussi H, Medintz IL. Delivering quantum dots into cells: strategies, progress and remaining issues. Anal Bioanal Chem 2009;393:1091–105.Google Scholar

  • 81.

    Hild WA, Breunig M, Goepferich A. Quantum dots – Nano-sized probes for the exploration of cellular and intracellular targeting. Eur J Pharm Biopharm 2008;68153–68.Google Scholar

  • 82.

    Al-Hajaj NA, Moquin A, Neibert KD, Soliman GM, Winnik FM, Maysinger D. Short ligands affect modes of QD uptake and elimination in human cells. ACS Nano 2011;5:4909–18.CrossrefGoogle Scholar

  • 83.

    Medintz IL, Pons T, Delehanty JB, Susumu K, Brunel FM, Dawson PE, et al. Intracellular delivery of quantum dot–protein cargos mediated by cell penetrating peptides. Bioconjugate Chem 2008;19:1785–95.CrossrefGoogle Scholar

  • 84.

    Delehanty JB, Bradburne CE, Susumu K, Boeneman K, Mei BC, Farrell D, et al. Spatiotemporal multicolor labeling of individual cells using peptide-functionalized quantum dots and mixed delivery techniques. J Am Chem Soc 2011;133:10482–9.Google Scholar

  • 85.

    Xue FL, Chen JY, Guo J, Wang CC, Yang WL, Wang PN, et al. Enhancement of intracellular delivery of cdte quantum dots (QDs) to living cells by tat conjugation. J Fluoresc 2007;17:149–54.CrossrefGoogle Scholar

  • 86.

    Lei Y, Tang H, Yao L, Yu R, Feng M, Zou B. Applications of mesenchymal stem cells labeled with tat peptide conjugated quantum dots to cell tracking in mouse body. Bioconjugate Chem 2008;19:421–7.CrossrefGoogle Scholar

  • 87.

    Liu BR, Li J-F, Lu S-W, Lee H-J, Huang Y-W, Shannon KB, et al. Cellular internalization of quantum dots noncovalently conjugated with arginine-rich cell-penetrating peptides. J Nanosci Nanotechnol 2010;10:6534–43.CrossrefGoogle Scholar

  • 88.

    Delehanty JB, Medintz IL, Pons T, Brunel FM, Dawson PE, Mattoussi H. Self-assembled quantum dot–peptide bioconjugates for selective intracellular delivery. Bioconjugate Chem 2006;17:920–7.CrossrefGoogle Scholar

  • 89.

    Santra S, Yang H, Stanley JT, Holloway PH, Moudgil BM, Walter G, et al. Rapid and effective labeling of brain tissue using TAT-conjugated CdS:Mn/ZnS quantum dots. Chem Commun 2005;3144–6.CrossrefGoogle Scholar

  • 90.

    Johnston HJ, Hutchison G, Christensen FM, Peters S, Hankin S, Stone V. A review of the in vivo and in vitro toxicity of silver and gold particulates: particle attributes and biological mechanisms responsible for the observed toxicity. Crit Rev Toxicol 2010;40:328–46.CrossrefGoogle Scholar

  • 91.

    Liu L, Yang J, Xie J, Luo Z, Jiang J, Yang YY, et al. The potent antimicrobial properties of cell penetrating peptide-conjugated silver nanoparticles with excellent selectivity for Gram-positive bacteria over erythrocytes. Nanoscale 2013;5:3834–40.CrossrefGoogle Scholar

  • 92.

    Daniel M-C, Astruc D. Gold nanoparticles: assembly, supramolecular chemistry, quantum-size-related properties, and applications toward biology, catalysis, and nanotechnology. Chem Rev 2004;104:293–46.CrossrefGoogle Scholar

  • 93.

    Pissuwan D, Valenzuela SM, Cortie MB. Therapeutic possibilities of plasmonically heated gold nanoparticles. Trends Biotechnol 2006;24:62–7.CrossrefGoogle Scholar

  • 94.

    Lee J, Chatterjee DK, Lee MH, Krishnan S. Gold nanoparticles in breast cancer treatment: promise and potential pitfalls. Cancer Lett 2014;347:46–53.Google Scholar

  • 95.

    Alric C, Miladi I, Kryza D, Taleb J, Lux F, Bazzi R, et al. The biodistribution of gold nanoparticles designed for renal clearance. Nanoscale 2013;5:5930–9.CrossrefGoogle Scholar

  • 96.

    Zhao F, Zhao Y, Liu Y, Chang X, Chen C, Zhao Y. Cellular uptake, intracellular trafficking, and cytotoxicity of nanomaterials. Small 2011;7:1322–37.CrossrefGoogle Scholar

  • 97.

    Conde J, Ambrosone A, Sanz V, Hernandez Y, Marchesano V, Tian F, et al. Design of multifunctional gold nanoparticles forin vitroandin vivogene silencing. ACS Nano 2012;6: 8316–24.CrossrefGoogle Scholar

  • 98.

    Krpetic Z, Saleemi S, Prior IA, See V, Qureshi R, Brust M. Negotiation of intracellular membrane barriers by TAT-modified gold nanoparticles. ACS Nano 2011;5:5195–201.CrossrefGoogle Scholar

  • 99.

    Oh E-K, Delehanty JB, Sapsford KE, Susumu K, Goswami R, Blanco-Canosa JB, et al. Cellular uptake and fate of PEGylated gold nanoparticles is dependent on both cell-penetration peptides and particle size. ACS Nano 2011;5:6434–48.CrossrefGoogle Scholar

  • 100.

    Ryan JA, Overton KW, Speight ME, Oldenburg CN, Loo L, Robarge W, et al. Cellular uptake of gold nanoparticles passivated with BSA–SV40 large T antigen conjugates. Anal Chem 2007;79:9150–9.Google Scholar

  • 101.

    Tkachenko AG, Xie H, Liu Y, Coleman D, Ryan J, Glomm WR, et al. Cellular trajectories of peptide-modified gold particle complexes: comparison of nuclear localization signals and peptide transduction domains. Bioconjugate Chem 2004;15:482–90.CrossrefGoogle Scholar

  • 102.

    Kumari A, Yadav SK, Yadav SC. Biodegradable polymeric nanoparticles based drug delivery systems. Colloids Surf, B 2010;75:1–18.CrossrefGoogle Scholar

  • 103.

    Hans ML, Lowman AM. Biodegradable nanoparticles for drug delivery and targeting. Curr Opin Solid State Mater Sci 2002;6:319–27.Google Scholar

  • 104.

    Jabbari E, Yang X, Moeinzadeh S, He X. Drug release kinetics, cell uptake, and tumor toxicity of hybrid VVVVVVKK peptide-assembled polylactide nanoparticles. Eur J Pharm Biopharm 2013;84:49–62.CrossrefGoogle Scholar

  • 105.

    Zhang K, Fang H, Chen Z, Taylor J-S, Wooley KL. Shape effects of nanoparticles conjugated with cell-penetrating peptides (HIV Tat PTD) on CHO cell uptake. Bioconjugate Chem 2008;19:1880–7.CrossrefGoogle Scholar

  • 106.

    Bain CD, Troughton EB, Tao YT, Evall J, Whitesides GM, Nuzzo RG. Formation of monolayer films by the spontaneous assembly of organic thiols from solution onto gold. J Am Chem Soc 1989;111:321–35.CrossrefGoogle Scholar

  • 107.

    Love JC, Estroff LA, Kriebel JK, Nuzzo RG, Whitesides GM. Self-assembled monolayers of thiolates on metals as a form of nanotechnology. Chem Rev 2005;105:1103–69.CrossrefGoogle Scholar

  • 108.

    Brust M, Walker M, Bethell D, Schiffrin DJ, Whyman R. Synthesis of thiol-derivatised gold nanoparticles in a two-phase Liquid-Liquid system. J Chem Soc, Chem Commun 1994:801–2.CrossrefGoogle Scholar

  • 109.

    Hou W, Dasog M, Scott RW. Probing the relative stability of thiolate- and dithiolate-protected Au monolayer-protected clusters. Langmuir 2009;25:12954–61.CrossrefGoogle Scholar

  • 110.

    Zhao Y, Perez-Segarra W, Shi Q, Wei A. Dithiocarbamate assembly on gold. J Am Chem Soc 2005;127:7328–9.CrossrefGoogle Scholar

  • 111.

    Walter M, Akola J, Lopez-Acevedo O, Jadzinsky PD, Calero G, Ackerson CJ, et al. A unified view of ligand-protected gold clusters as superatom complexes. Proc Natl Acad Sci USA 2008;105:9157–62.CrossrefGoogle Scholar

  • 112.

    Cheng Y, Meyers JD, Broome A-M, Kenney ME, Basilion JP, Burda C. Deep penetration of a PDT drug into tumors by noncovalent drug-gold nanoparticle conjugates. J Am Chem Soc 2011;133:2583–91.Google Scholar

  • 113.

    Levy R, Thanh NT, Doty RC, Hussain I, Nichols RJ, Schiffrin DJ, et al. Rational and combinatorial design of peptide capping ligands for gold nanoparticles. J Am Chem Soc 2004;126:10076–84.CrossrefGoogle Scholar

  • 114.

    Flynn NT, Tran TN, Cima MJ, Langer R. Long-term stability of self-assembled monolayers in biological media. Langmuir 2003;19:10909–15.CrossrefGoogle Scholar

  • 115.

    Taylor U, Rehbock C, Streich C, Rath D, Barcikowski S. Rational design of gold nanoparticle toxicology assays: a question of exposure scenario, dose and experimental setup. Nanomedicine 2014;9:1971–89.CrossrefGoogle Scholar

  • 116.

    Lelle M, Peneva K. An amino acid-based heterofunctional cross-linking reagent. Amino Acids 2014;46:1243–51.CrossrefGoogle Scholar

  • 117.

    Streich C, Koenen S, Lelle M, Peneva K, Barcikowski S. Influence of ligands in metal nanoparticle electrophoresis for the fabrication of biofunctional coatings. Appl Surf Sci 2015; doi:10.1016/j.apsusc.2014.12.159.CrossrefGoogle Scholar

  • 118.

    Khullar P, Singh V, Mahal A, Dave PN, Thakur S, Kaur G, et al. Bovine serum albumin bioconjugated gold nanoparticles: synthesis, hemolysis, and cytotoxicity toward cancer cell lines. J Phys Chem C 2012;116:8834–43.CrossrefGoogle Scholar

  • 119.

    Selvan ST, Tan TT, Yi DK, Jana NR. Functional and multifunctional nanoparticles for bioimaging and biosensing. Langmuir 2010;26:11631–41.CrossrefGoogle Scholar

  • 120.

    Susumu K, Uyeda HT, Medintz IL, Pons T, Delehanty JB, Mattoussi H. Enhancing the stability and biological functionalities of quantum dots via compact multifunctional ligands. J Am Chem Soc 2007;129:13987–96.Google Scholar

  • 121.

    Wei Y, Jana NR, Tan SJ, Ying JY. Surface coating directed cellular delivery of TAT-functionalized quantum dots. Bioconjugate Chem 2009;20:1752–8.CrossrefGoogle Scholar

Supplemental Material

The online version of this article (DOI 10.1515/bnm-2015-0001) offers supplementary material, available to authorized users.

About the article

Corresponding author: Kalina Peneva, Max Planck Institute for Polymer Research, Ackermannweg 10, 55128 Mainz, Germany, Phone: +(49) 6131 379136, E-mail:

Received: 2015-01-05

Accepted: 2015-01-09

Published Online: 2015-05-21

Published in Print: 2015-03-01

Citation Information: BioNanoMaterials, Volume 16, Issue 1, Pages 59–72, ISSN (Online) 2193-066X, ISSN (Print) 2193-0651, DOI: https://doi.org/10.1515/bnm-2015-0001.

Export Citation

©2015 by De Gruyter.Get Permission

Supplementary Article Materials

Citing Articles

Here you can find all Crossref-listed publications in which this article is cited. If you would like to receive automatic email messages as soon as this article is cited in other publications, simply activate the “Citation Alert” on the top of this page.

Razieh P. Ahwazi, Melika Kiani, Meshkat Dinarvand, Akram Assali, Farnaz S. M. Tekie, Rasoul Dinarvand, and  Fatemeh Atyabi
Journal of Cellular Physiology, 2019
Marco Lelle, Christoph Freidel, Stefka Kaloyanova, Klaus Müllen, and Kalina Peneva
International Journal of Peptide Research and Therapeutics, 2017
Manu S. Singh, Salma N. Tammam, Maryam A. Shetab Boushehri, and Alf Lamprecht
Pharmacological Research, 2017
Marco Lelle, Christoph Freidel, Stefka Kaloyanova, Ilja Tabujew, Alexander Schramm, Michael Musheev, Christof Niehrs, Klaus Müllen, and Kalina Peneva
European Journal of Medicinal Chemistry, 2017, Volume 130, Page 336
Johannes Franz, Marco Lelle, Kalina Peneva, Mischa Bonn, and Tobias Weidner
Biochimica et Biophysica Acta (BBA) - Biomembranes, 2016, Volume 1858, Number 9, Page 2028

Comments (0)

Please log in or register to comment.
Log in