PDF

Theranostics 2022; 12(17):7509-7531. doi:10.7150/thno.77259 This issue Cite

Review

Lipid nanoparticles for delivery of RNA therapeutics: Current status and the role of in vivo imaging

Han Na Jung^1*, Seok-Yong Lee^2,4,5*, Somin Lee³, Hyewon Youn^4,5 , Hyung-Jun Im^1,3,4,6

1. Department of Applied Bioengineering, Graduate School of Convergence Science and Technology, Seoul National University, Seoul 08826, Republic of Korea.
2. Department of Biomedical Sciences, Seoul National University Graduate School, Seoul 03080, Republic of Korea.
3. Department of Molecular Medicine and Biopharmaceutical Sciences, Graduate School of Convergence Science and Technology, Seoul National University, Seoul 08826, Republic of Korea.
4. Cancer Research Institute, Seoul National University College of Medicine, Seoul 03080, Republic of Korea.
5. Department of Nuclear Medicine, Seoul National University Hospital, Seoul 03080, Republic of Korea.
6. Research Institute for Convergence Science, Seoul National University, Seoul, 08826, Republic of Korea.
* These authors contributed equally to this work.

✉ Corresponding authors: Dr. Hyung Jun Im, iiihjjjac.kr; Dr. Hyewon Youn, hwyounac.kr

Abstract

Lipid nanoparticles (LNPs) have been one of the most successful nano-delivery vehicles that enable efficient delivery of cytotoxic chemotherapy agents, antibiotics, and nucleic acid therapeutics. During the coronavirus disease (COVID-19) pandemic, LNP-based COVID-19 messenger RNA (mRNA) vaccines from Pfizer/BioNTech and Moderna have been successfully developed, resulting in global sales of $37 billion and $17.7 billion, respectively, in 2021. Based on this success, the development of multiple LNP-based RNA therapeutics is gaining momentum due to its potential in vaccines and therapeutics for various genetic diseases and cancers. Furthermore, imaging techniques can be utilized to evaluate the pharmacokinetics and pharmacodynamics (PK/PD) effects, which helps target discovery and accelerates the development of LNP-based mRNA therapies. A thorough introduction and explanation of the components of LNPs and its functions along with various production methods of formulating LNPs are provided in this review. Furthermore, recent advances in LNP-based RNA therapeutics in clinics and clinical trials are explored. Additionally, the evaluation of PK/PD of LNPs for RNA delivery and the current and potential roles in developing LNP-based mRNA pharmaceutics through imaging techniques will be discussed.

Keywords: Lipid nanoparticles, RNA therapeutics, Drug delivery system, Vaccines, In vivo imaging

Introduction

RNA therapeutics have shown potential in various medical applications, including virus vaccines, cancer immunotherapy, and gene editing [1]. The various drug delivery vehicles including lipid nanoparticles (LNP) for RNA therapeutics have been developed because of the instability of RNA. In 1978, the delivery of mRNA using liposomes was first reported [2]. To further improve the encapsulation of the charged mRNA, cationic lipid based LNPs [3] and ionizable lipid based LNPs [4] were sequentially developed. Currently, ionizable lipids are considered as crucial components of LNP-based RNA therapeutics because they are positively charged at a low pH to enhance the encapsulation of negatively charged RNA, and the charge becomes less positive or almost neutral at physiological pH (~7.4), to reduce the toxicity [5]. In addition, various mRNA engineering methods have been developed to enhance the stability and the translation efficacy of mRNA therapeutics, such as a selection of untranslated regions (UTRs), addition of a poly-A tail, capping, and nucleoside modification [6]. Based on these advanced techniques, two LNP-based mRNA vaccines (BNT 162b2, Pfizer-BioNTech; and mRNA-1273, Moderna) were successfully developed and obtained authorization from regulatory agencies in 2020 in multiple countries [7]. Additionally, multiple types of LNP-based RNA therapeutics are under active investigation to treat various infectious diseases and cancers [8].

Bioimaging has a crucial role in identifying drug targets and evaluating off-target effects and pharmacokinetics/pharmacodynamics (PK/PD) profiles of drugs [9, 10]. Nanoparticles are considered as a suitable platform to utilize bioimaging because it is easy to incorporate various types of imaging contrasts in the nanoparticles which do not significantly affect their PK characteristics [11]. Furthermore, the development of bioimaging techniques for therapeutics can result in the development of theranostic agents. The theranostic approach has drawn attention to the development of drugs due to the following advantages: 1) In the preclinical stage, it can help to select appropriate drug candidates based on the imaging results; 2) in clinical trials, companion imaging methods can be used to select patients for enrollment in clinical trials; 3) finally, in clinical practice, unnecessary treatment can be avoided by using companion imaging biomarkers for patient selection. With these benefits, theranostic agents have been successfully developed in recent years. For example, the U.S. Food and Drug Administration (FDA) approved ¹⁷⁷Lu-dotatate (Lutathera) in neuroendocrine tumors and ¹⁷⁷Lu-PSMA-617 (Pluctivo) in prostate cancer [12]. Additionally, numerous studies have been conducted to develop theranostic nanoparticles because 1) nanoparticles can be functionalized with therapeutics and diagnostics easily and 2) various methods for controlled release of the therapeutics can be applied [13, 14].

This review presents a comprehensive description of the currently available LNP production methods for LNP-based RNA therapeutics and LNP-based RNA therapeutics in clinics and clinical trials, and the PK/PD characteristics of LNP-based RNA therapeutics and the current and potential roles of imaging techniques in the development of LNP-based RNA therapeutics as shown in Figure 1.

Development of LNP for RNA Delivery

Lipid nanoparticle compositions

The idea of using mRNA as a novel therapeutic drug first took place in 1989 by Vical Incorporated a start-up company in San Diego. The company first published its research demonstrating mRNA encapsulation into liposomes and succeeded in transfecting mRNA into various eukaryotic cells [15]. Afterwards, various studies have been done to properly deliver mRNA across the cell membrane into cytosol, because mRNA directs the synthesis of proteins in the cytoplasm using various nanoparticles such as polymeric particles and liposomes [2, 16, 17]. Recently, the use of LNPs as mRNA delivery vehicles has become a leading technology in the application of vaccines [18-20]. Loading mRNAs into LNPs is stable, leading to a successful delivery into cells [21]. The LNPs typically consist of four different components with a unique role shown in both Figure 2 and Table 1.

 Figure 1 

Overall schematic illustration of lipid nanoparticles for delivery of RNA therapeutics.

 Figure 2 

Illustration of lipid nanoparticle and its compositions. Created with BioRender.com.

Ionizable lipids

The ionizable lipids determine the potency of the LNP because it has a crucial role in encapsulating mRNA or other different types of nucleic acids [22]. In general, cationic lipids contain alkylated quaternary ammonium groups for which the charge of the lipids remains the same in different pH. On the other hand, ionizable lipids form a positive charge at a low pH (<6.0) because the free amine is protonated as the pH decreases. When the pH changes back to physiological condition (pH ~7.4), the charge of the ionizable lipids becomes less positive or neutral [23, 24]. This characteristic of ionizable lipids offers several major advantages in the delivery of mRNA. First, the switching of the lipid charge at a different pH enables a high encapsulation efficiency of the mRNA because the positive charge of the lipid interacts with the anionic mRNA at a low pH [25-28]. Therefore, formulating LNPs using ionizable lipids offers less positive or neutral charge at a physiological pH, which not only enhances the biocompatibility of the nanoparticles but also helps prevent the nonspecific binding of anionic biomolecules [26]. The capability of the change in charge of the ionizable lipids depending on the environmental pH is recognized as a key component of the endosomal escape of LNPs. As endosomal maturation begins, the low pH inside the endosome turns ionizable lipids to a positive charge. These positively charged ionizable lipids interact with the negatively charged inner endosome membrane forming a non-bilayer structure of a hexagonal (H_II) phase. As membrane fusion occurs, the entrapped nucleic acids in the LNPs escape and are released into the cytosol [29]. However, it has been reported that less than 2-3% of nucleic acids escape from the endosome and are released into the cytosol [30, 31]. Therefore, improving the percentage of RNA release into the cytosol is one of the keys to open the full potential of LNPs.

Phospholipids and cholesterol

The other components of LNPs are the “helper lipids,” which are phospholipids (i.e., DSPC, DOPE, etc.) and cholesterol. In general, these helper lipids not only provide structural stability of the nanoparticle, which improve the biodistribution of LNPs and enhance the delivery efficacy by promoting intracellular uptake and cytosolic entry [32, 33]. Additionally, depending on the types of phospholipids, it can lead to disruption of the lipid bilayer, which promotes endosomal escape [34-38].

One of the commonly used phospholipids is a phosphatidylcholine (PC), such as 1,2-distearyol-sn-glycero-3-phosphocholine (DSPC) and hydrogenated soybean PC (HSPC). DSPC is clinically applied such as siRNA therapeutics (Patisiran) and mRNA vaccines against SARS-CoV-2 (mRNA-1273 and BNT126b2) [5, 33]. DSPC contains a saturated acyl chains, containing one or more double bonds, in the tail of the lipid and a relatively larger head group, which forms a cylinder-shaped geometry. Furthermore, the high melting temperatures (T_m) value of this lipid provides highly stable LNP structure [39-41]. Due to its high stability, it inhibits membrane fusion with the endosomal membrane, which inhibits endosomal escape. On the other hand, DOPE is considered as a fusogenic lipids. It contains two unsaturated acyl chains, containing hydrocarbon chain with single bond only, in the tail and relatively smaller head group, which forms cone-shape geometry [39, 42]. These unsaturated acyl chain lipids have low melting temperature (T_m) values and stabilize the non-bilayer hexagonal II (H_II) phase. In the physiological temperature, DOPE forms a non-lamellar lipid phase due to the inverted hexagonal (H_II) phase. This enables membrane fusion, bilayer disruption, that leads to endosomal escape [36, 43, 44]. Additionally, DOPE is reported to enhance the transfection efficacy when present in cationic lipid formulations by facilitating membrane fusion [44-46].

Cholesterol is also used in LNP development as it enhances particle stability by regulating membrane integrity and rigidity [33]. According to Patel et al., cholesterol has an important role in enhancing gene transfection and biodistribution of mRNA-LNPs due to the analog with C-24 alkyl phytosterols. Therefore, the study by Patel et al. reports that maintaining high transfection requires 1) the polarity of the hydroxyl group, 2) the sterol ring flexibility, and 3) length of alkyl tail [47]. Kotoucek et al. also provide an insight into the role of cholesterol in the formulation of liposomes by formulating liposomes with various molar ratios of cholesterol. Because cholesterol was mixed with DSPC with an increasing molar ratio (10 ~ 50 mol %), the liposome size decreased, indicating the amount of cholesterol affects the size of the liposomes [48].

PEGylated lipids

The PEGylated lipids have various roles in LNP formulations and mRNA delivery [49-52]. The structure of the PEGylated lipids contains a hydrophilic head and hydrophobic tail. The PEGylated lipids have a wide molar mass range from 400 Da to 50 kDa. Therefore, it is important to use an appropriate molar mass according to the application. The amount of PEGylated lipids in LNP formulations determines the size and zeta potential, which are also important properties that affect the delivery efficacy [50]. The large molar mass of PEG, such as 20 to 50 kDa, is applied in the usage of drugs with low molar mass (e.g. oligonucleotides, siRNA, small molecules, etc.). The use of a large molar mass of PEG increases the size of the drug carrier, enabling it to avoid renal clearance. On the other hand, a lower molar mass of PEG, such as 1 to 5 kDa, is used in larger drugs: antibodies and nanoparticle drugs [49].

Furthermore, there are many research reports that PEGylated lipids enhance stability and decrease the aggregation of LNPs [27, 33, 49]. Thus, PEGylated lipids enhance the blood circulation time and protect the LNPs surface, decreasing the kidney's clearance. PEGylated lipids also protect LNPs from uptake by the mononuclear phagocyte system (MPS) [51-53]. As PEGylated lipids prevent aggregation and control the size of LNPs, they overall increase the stability with a potential decrease of ApoE adsorption and particle fusogenicity [54-57]. The “stealth effect” through PEGylated lipids decreases protein adsorption and the cellular uptake and transfection capacity of LNPs [58]. To overcome this so-called “PEG-dilemma,” the length of PEGylated lipids needs to be considered as the shorter acyl chains (C8-14) quickly spread out of the LNP than the longer acyl chains (C16-C24), which achieve a higher transfection efficiency [59-63].

Though PEGylated lipids are one of the crucial and useful components of LNPs, PEG immunogenicity and anti-PEG antibodies need to be considered in developing LNP-based vaccines and therapeutics. According to recent studies, both SARS-CoV-2 mRNA LNP-based vaccines, mRNA-1273 (Moderna) and BNT126b2 (Pfizer/BioNTech), induced the amount of anti-PEG IgM and anti-PEG IgG in human samples [64, 65]. Both studies show a common detection of anti-PEG antibodies before the vaccination due to previous exposure to PEG from cosmetics and PEG-containing medicines. However, both mRNA-1273 and BNT126b2 vaccines significantly induced anti-PEG IgM and anti-PEG IgG after the administration. Furthermore, studies showed that mRNA-1273 induced more anti-PEG antibodies than BNT126b2. This result could have been affected by several reasons. 1) The type of PEG's terminal group and 2) the shedding rate of PEGylated lipids from LNPs [65-67]. There are different terminal groups of PEG, such as methoxy, hydroxy, etc. Clinically, most PEGylated drugs use methoxy terminal group PEG (mPEG). Compared to hydroxy-PEG (HO-PEG), mPEG induces higher PEG immunogenicity [64-66, 68]. Also, most PEG-specific antibodies identify the repeated ethylene oxide subunits, the backbone of the molecules. Although both mRNA-1273 and BNT162b2 apply different PEG structures, they both contain methoxy terminal group PEG. Therefore, it is unlikely the structure of the PEG that affects the inducing amount of anti-PEG antibodies but rather the higher dose of mRNA-1273 (100 μg) administered compared to BNT126b2 (30 μg). Another factor that causes PEG immunogenicity is the shedding rate of PEG [67-69]. The anti-PEG antibodies are induced depending on the shedding rate of the PEGylated lipid from LNPs. The shedding rate is dependent on the length of the acyl chain. A short acyl chain leads to fast shedding of LNP, which induces less PEG immunogenic, whereas a longer acyl chain leads to slower shedding, which induces a more immunogenic response [67, 69]. Several studies mentioned regard to PEG immunogenicity and anti-PEG antibodies. There is still a need for clinical relevance in PEG-specific antibodies induced by mRNA LNP-based medications and vaccines, as well as exploring an alternative to PEG in developing mRNA LNP-based vaccines and therapeutics.

Various production methods for LNPs

Thin-film hydration

Cationic liposomes were the first delivery carrier used in mRNA vaccines [18]. Thin-film hydration or the Bangham method is one of the most commonly used techniques for liposome production [70]. This passive encapsulation approach is produced as the phospholipids spontaneously self-assemble into vesicles [71, 72]. Because the lipids are dissolved in an organic solvent, such as ethanol or chloroform, the lipids are then evaporated through a rotary evaporator, leading to a thin lipid layer formation. As the thin layer is hydrated using an aqueous buffer solution loaded with nucleic acids, the hydrophobic and hydrophilic parts of the lipids are self-assembled. Thus, it leads to the formulation of large multilamellar vesicles (MLVs) that are very heterogeneous with a size of micrometers [73, 74]. The advantages of using thin-film hydration methods are 1) it is the simplest production procedure to prepare, 2) it does not involve in using expensive, complex lab equipment, and 3) high pressure or temperature is not needed in maintenance.

 Figure 3 

Illustration of various LNP production methods. Created with BioRender.com.

However, the size of the vesicles must be reduced and homogenized through extrusion or sonication of the MLVs to form small or large unilamellar vesicles (SUVs and LUVs) for effective therapeutic administration [75-77]. The extrusion process to reduce the size of the vesicles is done by repeatedly forcing the heterogeneous suspension through a filter of the desired size. Sonicators (probe or bath) is another method used to reduce the vesicle size. However, sonication for size reduction provides less control over the size result than extrusion [78, 79]. Though this method is commonly used in vesicle production, the complex steps of the manufacturing method and its labor-intensiveness make this production lack scalability and result in high costs [80-82]. Another limitation of using the thin-film hydration method is the low encapsulation efficiency in general. An excess amount of lipids is used in the production process to improve the encapsulation efficiency, which leads to an increase in the cost and toxicity [79]. As the batch size increases, the volume of the organic solvent will also increase, which would take several hours to evaporate the organic solvent, making it time-consuming at a large scale [71]. In addition, a mass amount of production would be difficult using extruders, which may lead to filter tears and clogging of the membrane that will result in a large batch failure and product loss [80].

Ethanol injection

Ethanol injection is another general technique that forms unilamellar liposomes. In this method, lipids are dissolved in ethanol and injected at a fast rate into an aqueous buffer under stirring, containing drug or the compound for encapsulation, where the volume is relatively higher than the lipid solution, rapidly forms vesicles [83, 84]. One of the advantages of using ethanol injection methods is the simple and convenient procedure. Gouda et al. reports the production of homogenous SUVs can be formulated when the ethanol percentage is less than 7.5% of the total volume (v/v) through ethanol injection method [84]. This production method is one of the earliest alternatives to the thin-film hydration method, in which a sonication procedure is not needed [83]. This technique was first introduced and developed in 1973 by Batzri and Korn [85]. The self-arranged vesicles are formed as the injected lipid solutions are quickly diluted with an aqueous buffer due to the increase of polarity in the mixed solvent. The size of these vesicles is controlled through the lipid concentration, stirring rate, injection rate, and the types of lipids used [85].

The other type of ethanol injection method called “crossflow injection” was developed as another way for the use of the mass production of liposomes [84]. This alternative device consists of two stainless steel tubes in a cross-shaped form with a small injecting hole at the intersection between the tubes. Through the crossflow tube, the ethanolic solution containing lipids is injected into a buffer solution by changing the pressure of the nitrogen regulator device forming liposomes. These various ethanol injection methods use high lipid concentrations, and these manufacturing production methods are not generally used due to the large size of heterogeneous nanoparticle production and low mRNA encapsulation efficiency [86]. Additionally, reproducibility on a large scale is challenging to accomplish because the use of the sonication procedure can degrade lipids and drug contents. The degradation of lipids and drug contents were reported as the samples are overheated through the sonication procedure [85, 87].

Nevertheless, these conventional liposomal methods mentioned are still widely used due to their simple implementation [88]. However, the lack of reproducibility, scalability and encapsulation efficiency holds them back from progressing further into clinical translation efficiency [89]. New production methods have been reported to overcome these challenges, which will be discussed below.

T-junction mixing

A lipid-based drug produced by T-junction mixing was introduced by Hirota et al. in 1999 [90]. Compared to the macroscopic mixing methods such as vortexing and pipetting, T-junction mixing produces reproducible and controllable nucleic acid-loaded lipoplexes [91]. Therefore, this method is the general choice for large batches of mRNA-LNPs for commercial production. T-junction produces rapid mixing through the injection of two different solvents as each inlet collides, which causes a turbulent flow. Moreover, the constant speed of the mixture is important. Though there are limited data on the different factors that could influence the formulation of LNPs, Kulkarni et al. demonstrated the flow rate ratio of the mixing solution influences the size and PDI value when formulating LNPs [92]. In that study, T-junction mixing was used to produce LNPs encapsulating inorganic hydrophobic nanoparticles, iron oxides. The results show that the size of the LNP decreased with the increase in the total flow rate. When the total flow rate was 10 mL min^-1, the size of the LNP was observed to be 75 6 nm, while the size of the LNP was 36 2 nm when the total flow rate was 40 mL min^-1. The value of PDI was also affected by the flow rate because the PDI value was higher at a lower flow rate compared to the low value of the PDI at a higher flow rate [93]. This result indicates that the control of the flow using T-junction mixing can impact the characteristics of the nanoparticle formulation.

Though there are few productions of mRNA-LNPs using T-junction mixing at the laboratory scale, there are some studies are being done regards to the encapsulation efficiency as well as the particle formulation size and morphology. Goswami et al. used mannosylated lipid nanoparticles to potentially enhance the uptake by antigen-presenting cells (APCs) and encapsulated mRNA [94]. The LNPs were composed of DSPC, cholesterol DLin-DMA and DMG-PEG2000 (10:48:40.2 mol %) and prepared in ethanol. The ethanol dilution method using T-junction was used. Then the lipid content in ethanol was mixed with mRNA in a 100 mM citrate buffer (pH 6) with a nitrogen to phosphate (N/P) ratio of 8. The resulting size of the particles was 129.9 0.98 nm with a 0.1 PDI value. The resulting encapsulation efficiency was 88.40 %, successfully encapsulating 11.78 μg mL^-1 of the mRNA. Additionally, Chen et al. demonstrated a similar T-junction mixing setup to formulate LNPs with various encapsulated nucleic acids, such as CpG, siRNA, mRNA, and pDNA [95]. For the mRNA encapsulation, DLin-MC3-DMA, DSPC, cholesterol, and PEG-DMG (50:10:38.5:1.5 mol %) were dissolved in ethanol and mixed with mRNA dissolved in 25 mM acetate buffer at pH 4 through T-junction mixing. The ethanolic and aqueous solutions were mixed at a 1:3 (v/v) ratio with a final flow rate of > 10 mL min^-1. The exact size and the encapsulation efficiency of the nanoparticles were mentioned. However, it was indicated that the range of the nanoparticle sizes was 46 ~ 50 nm with a PDI value less than 0.1. It was also mentioned that LNPs exhibiting < 86 % nucleic acid entrapment were not used for the further experiments [95]. Lazzaro et al. also applied T-junction mixing in their fabrication of mRNA-LNPs for CD8 T-cell priming upon self-amplifying mRNA vaccination. In this experiment, mRNA was encapsulated with DLin-DMA, DSPC, PEG-DMG2000, and cholesterol (40:10:2:48 mol %) with an N/P ratio of 8 using T-junction mixing. The resulting nanoparticle sizes were < 200 nm with a PDI value < 0.15. The encapsulation efficiency was > 85% [96, 97].

These previous works show that mRNA-LNPs can be formulated using T-junction mixing. This method generally offers a higher encapsulation efficiency than encapsulation through conventional liposomal methods. However, the high flow rate requirement for rapid mixing through T-junction is not preferred on a laboratory scale but for large-scale production. Moreover, the mixture is dependent on the channel length and the contact surface area. Therefore, the decreased influence of mass transport can be caused by a short mixing time by T-junction mixing, which leads to lipid aggregation and heterogeneity of the nanoparticle formulation [98]. Though there are several reports on LNP production through T-junction mixing, further studies are needed on identifying the various factors that affect the LNP formulation.

Microfluidic mixing

Typical operating microchannel conditions have a laminar flow with slow molecular diffusion through the channel. The absence of a turbulent flow makes it difficult to mix solutions effectively. That is why the addition of the staggered-herringbone structure to the fluidic channel was implemented and introduced by Stroock et al. in 2002 [99]. Compared to the simple and smooth channel of a typical microchannel, the additional structure to the fluidic channel promotes the reduction of hydrodynamic dispersion, enabling an effective mixing of solutions. This chaotic mixing method of microfluidics was pioneered in developing LNPs by the Pieter Cullis research group and later commercialized by Precision Nanosystem [23, 100, 101]. Additionally, it has been reported that staggered-herringbone structured microfluidic chips can be simply extensible to produce large batches [102]. The development of pattern structured microfluidic chips has improved the control of the mixing procedure leading to the control of homogenous particle size and distribution and a higher encapsulation compared to the bulk methods [103]. The rapid mixing offered through the staggered-herringbone structure suddenly increases the polarity of a mixture, which causes supersaturation that results in LNP formation [103, 104]. It has been reported that controlling the total flow rate (TFR) and the flow rate ratio (FRR) can affect the size and the size distribution of the LNPs, for which the structured microfluidic chip is a suitable application in LNP production [100, 103, 105]. Recently, Moderna has reported the size regulation of mRNA-LNPs through TFR control [106, 107]. The mRNA-LNP was formulated using the novel synthesized ionizable lipid H. Lipid H, DSPC, cholesterol, and PEG2k-DMG with molar ratios of 50:10:38.5:1.5 were dissolved in ethanol mixed with mRNA buffer solution through a microfluidic system at different TFRs. The TFRs ranged from 0.5 mL min^-1 to 12 mL min^-1, and it was observed that the particle size decreased as the TFR was increased. Furthermore, Shepherd et al. have also demonstrated the scalable production of mRNA and siRNA LNPs using a parallelized microfluidic device (PMD) [102]. The PMD contains an array of 128 mixing channels that simultaneously operate. It can produce over a 100-fold production rate compared to a single-channel microfluidic chip. The mRNA-LNPs produced by PMD contain C12-200, DOPE, cholesterol, and PEGylated lipid with luciferase mRNA at a flow rate of 18.4 L h^-1. The results showed the ability to reproduce the size of the mRNA-LNPs that were > 140 nm with a low polydispersity.

Though there are many advantages of both T-junction and microfluidic mixing, one of the drawbacks is the requirement of a large amount of organic solvent in manufacturing production as shown in Table 2. Additionally, using ethanol to dissolve lipids can bring about limitations in the types of lipids chosen [23]. Regardless, LNP production through microfluidic mixing methods became a major platform encapsulating various types of nucleic acids such as siRNA and mRNA. There are various microfluidic chip designs and different particle formulations, making it difficult to compare directly. However, the rapid mixing production methods such as T-junction and microfluidic devices have accomplished efficient and reproducible mRNA-LNPs. Scalability can be easily accomplished from a small laboratory to a large manufacturing scale [102]. Therefore, the production of mRNA-LNPs through microfluidic mixing has shown potential for opening a new pathway for nucleic acid-based therapeutics.

Recent advances in LNP-based RNA therapeutics in clinics or clinical trials

Clinical stage LNP-based RNA therapeutics

As various gene therapies enter clinical trials, LNPs have been considered as the most optimized and applicable delivery system for nucleic acids such as siRNA and mRNA because negatively charged nucleic acids interfere with the delivery to cell membranes and are degraded by endogenous nucleases in the body, making efficient delivery difficult without the aid of LNPs [88, 108]. Patisiran (ONPATTRO®), the first Food and Drug Administration (FDA) approved LNP-formulated siRNA drug, has reduced the formation of transthyretin protein in the liver and has been used to treat hereditary transthyretin-mediated amyloidosis since 2018. Amine head groups of the ionized lipid by 4-(diethylamino)-butanoic acid (DLin-MC3-DMA) optimized for siRNA delivery has had an important role in the drug [70]. Givosiran (GIVLAARI^TM), which received FDA approval in 2019, is a siRNA that targets the ALAS1 gene in hepatocytes and is prescribed for patients with the hereditary disease acute hepatic porphyria [109, 110]. The most recent topic is the Severe Acute Respiratory Syndrome Coronavirus 2 (SARS-CoV-2) infection, declared a pandemic by the World Health Organization (WHO). Representatively, Pfizer and BioNTech's BNT162b2 and Moderna's mRNA-1273 are LNP-formulated mRNA vaccines that have received emergency use authorization (EUA) by the FDA in December 2020. Most recently, on August 23, 2021, Pfizer/BioNTech's BNT162b2 was formally approved by the FDA for people 16 years of age or older or by the European Medicines Agency (EMA) for people 12 years of age or older with the official name “Comirnaty” (mRNA vaccine for COVID-19). Additionally, on January 31, 2022, Moderna's mRNA-1273 was the second approval of a mRNA vaccine for COVID-19 by the FDA for people 18 years of age and older or by the EMA for people 6 years of age and older with the official name “Spikevax”.

mRNA vaccine platforms

Unlike DNA-based vaccines, mRNA vaccines have less potential risk of insertional mutagenesis because mRNA vaccines are non-infectious, non-integrating platforms when compared to conventional vaccine platforms containing subunits, attenuated, inactivated, and killed pathogens. In vitro transcribed mRNA (IVT mRNA) is emerging as a potential replacement for conventional vaccines due to its advantages of faster, cheaper, and scalable manufacturability due to its more stable, translatable, and high yield productivity after transcriptional reactions [19]. The developed IVT mRNA is composed of four structurally modified forms to optimize its high translation efficiency and stability: 1) 5'-cap, 2) poly(A) tail, 3) 5' or 3'-untranslated regions (UTRs), 4) Open reading frame (ORF) [5, 111]. First, the 5'-cap modification mediates the binding of the decapping enzyme (DCPs) by attaching eukaryotic translation initiation factor 4E (EIF4E) to the cap analogues. Second, the poly(A) tail must be adjusted in length to affect the translational stability, and deadenylation is inhibited by recombinant poly(A) polymerase. Third, the 5'-UTR including internal ribosomal entry sites (IRES) improves the protein translation efficiency, and the 3'-UTR with an alpha or beta-globin sequence improves the IVT mRNA stability. Fourth, codon optimization in protein translation is known to be important for efficiency and acceleration. However, IVT mRNA has a limitation in direct clinical use due to the difficulty of cell membrane penetration from its anionic property [112]. Various clinical trials for mRNA-based vaccines are actively underway in infectious diseases [113], and other rare diseases.

 Figure 4 

Schematic mechanism of vaccine antigens with non-amplifying mRNA (namRNA) versus self-amplifying mRNA (samRNA). GOI: gene of interest; LNP: lipid nanoparticle; MHC: major histocompatibility complex; nsPn: non-structural polyprotein number.

Over the past decade, LNP formulations have been used to deliver various mRNA vaccine platforms. Typically, three types of RNA vaccine platforms have been used: self-amplifying messenger RNA (samRNA), non-amplifying messenger RNA (namRNA) vaccines [114] and circular RNA (circRNA) as shown in Figure 4.

The samRNA vaccine is based on the alpha virus genome and replaces the gene encoding “the antigen of interest” with the “the antigens of the vaccine” to generate a large amount of “the antigen of the vaccine” through intracellular replication by RNA replicon even with a very small amount of the mRNA vaccine [115]. Unlike samRNA, namRNA is a typical mRNA that is generally considered non-amplifying and does not have an RNA replicon. The namRNA was also used as a vaccine for infectious diseases or cancer and has economic advantages but has partial disadvantages in its low stability and ability to generate antigens, which are mRNA transcripts [19, 116]. Because samRNA is larger than namRNA and has an anionic charge, a cationic or ionizable LNP with a size of ~100 nm is used to facilitate cellular uptake and cytoplasmic release [26]. Clinical trials of samRNA vaccines are being actively conducted for various diseases. For the COVID-19 vaccine, the samRNA vaccine was first completed in a phase 1 / 2 clinical trial by the Imperial College London research team from 2020 to January 2021 (ISRCTN17072692). The benefits of samRNA were demonstrated using doses ranging from 0.1 to 10 μg, much smaller than the Pfizer/BioNTech (BNT162b2, 30 μg) and Moderna (mRNA-1273, 100 μg) vaccines. In addition, ARCT-021 from the Duke-NUS School of Medicine and Arcturus Therapeutics Inc., in a phase 1 / 2 clinical trial (NCT44800957), was found that multiple dose levels from 1 to 10 μg in healthy people aged 18 to 80 years, excluding pregnant and breastfeeding women, were evaluated as safe, tolerable, and immunogenic [116].

In addition, an RNA vaccine platform that is attracting attention is the single-stranded, loop-type circRNA. It is stable from nuclease-mediated degradation due to the lack of a 5'-cap or 3'-poly(A) tail, and has no stop codon, enabling continuous and high-efficiency protein translation [117, 118]. These circRNAs are already being used as targets for therapeutic approaches in various cancers, cardiovascular diseases, and central nervous system diseases [119].

mRNA-LNP vaccines for infectious diseases

As of September 07, 2022, multiple clinical trials for mRNA-LNP vaccines for various infectious diseases are ongoing with a total of 216 active (recruiting or not), suspended, terminated, withdrawn, or completed trials (https://clinicaltrials.gov/ct2/results?cond=Infectious+disease&term=mRNA+vaccine&cntry=&state=&city=&dist=). We summarized clinical trials with mRNA-LNP against infectious diseases as shown in Table 3.

Rabies

CureVAC AG RNAactive® CV7201 is a lyophilized, namRNA candidate vaccine encoding the rabies virus glycoprotein (RABV-G) and the ionizable cationic protein protamine. From October 2013 to January 2016, a dose of 80 to 640 μg of CV7201 was administered intradermally or intramuscularly by a needle syringe or needleless syringe device in 101 healthy people aged 18-40 years (NCT02241135). Seven days after vaccination, most showed local reactions and 78% systemic reactions. Needle-free delivery showed varying levels of neutralizing antibody induction, but the needle-syringe delivery did not [120]. Since October 2018, CureVAC AG's new mRNA-LNP, CV7202, has been undergoing a phase 1 clinical trial in 53 participants aged 18-40 years (NCT03713086). Two doses of 1 or 2 μg of CV7202 induced a higher rate of rabies-neutralizing antibody response than a single dose of 5 μg with a high reactogenicity in all recipients [121].

Influenza

Moderna's mRNA-1440 (VAL-506440) and mRNA-1851 (VAL-339851) are vaccines encoding from Haemagglutinin H10N8 and H7N9, respectively [122]. The inoculation of the mRNA-1440 vaccine administered as two doses of the vaccine 3 weeks apart showed 78.3% inhibition of haemagglutinin at 100 μg in healthy people aged 18-64 years (NCT03076385) and 96.3% inhibition by the inoculation of mRNA-1851 at 50 μg in healthy people aged 18-49 years (NCT03345043) [123].

Zika virus

Moderna's mRNA-1893 against Zika virus is an mRNA-LNP vaccine encoding the prM-E (pre-membrane and envelope) protein [124]. In a Phase 1 clinical trial conducted from 2019 to April 2020, a 100 μg dose level of mRNA-1893 induces a potent neutralizing Zika virus antibody response in both patients with and without flavivirus infection in 120 healthy people aged 18-49 years (NCT04064905). However, two dose levels (one-dose or two-dose schedules) of mRNA-1893 are being evaluated compared to a placebo in 800 healthy adults in a phase 2 trial based on the results initially observed at the 30 μg level in the phase 1 trial [125, 126].

Cytomegalovirus

Two mRNA vaccine candidates (mRNA-1647, mRNA-1443) against Cytomegalovirus (CMV) completed a phase 1 clinical trial from November 2017 to October 2020, in 181 healthy participants aged 18-49 years (NCT03382405). mRNA-1647 consists of six mRNAs of two antigens, five encode pentameric complexes and one encodes the full-length membrane-attached glycoprotein B, and mRNA-1443 encodes pp65 from T cells of the CMV antibody [127]. High neutralizing antibody responses (geometric mean titers, GMTs) in CMV seronegative and positive groups were achieved with excellent tolerability and no serious adverse effects 1 month after the third vaccination. Based on these results, in a phase 2 clinical trial, 452 healthy participants aged 18-40 years were vaccinated with 3 doses of 50, 100 and 150 μg once a month, respectively, in January 2020. Both the CMV seronegative and positive groups showed a dose-dependent increase in the neutralizing antibody GMT for 7 months after the first administration [128]. Based on this, mRNA-1647 (100 μg dose) entered a phase 3 clinical trial in 2021 [114].

 Figure 5 

Development and representative lipid compositions of the most advanced mRNA vaccines with COVID-19: Pfizer/BioNTech (BNT162b2) and Moderna (mRNA-1273).

SARS-CoV-2, COVID-19

In December 2019, COVID-19 was identified. There were no vaccines for COVID-19 infection, so the incidence and mortality rates began to accumulate rapidly [129, 130]. Therefore, as the clinical trials of new vaccines received urgent approval, various companies started developing the vaccine. Among them, Pfizer/BioNTech and Moderna reported that their mRNA vaccines against COVID-19 have shown a strong effect on disease prevention [131] seen in Figure 5. In the vaccines from both companies, the mRNAs encode the spike (S) protein of SARS-CoV-2 and translate into S proteins that serve as antigens and contribute to the development of the immune response of COVID-19.

In October 2020, Pfizer and BioNTech first validated the results of a comparative clinical trial of BNT162b1, encoding the receptor-binding domain (RBD) of the S protein in SARS-CoV-2, and BNT162b2, encodes a full-length S in an LNP formulated and nucleoside-modified RNA (modRNA). BNT162b2 showed a lower systemic reactivity and toxicity in 43,998 participants aged 18-85 years in the phase 1 clinical trial [132]. Two months later, on December 11, 2020, it was approved for EUA by the FDA, demonstrating a 95% efficacy and safety in participants aged 16-85 years through phase 2 and 3 clinical trials [133], including adolescents aged 12-15 years [134]. In pregnant women, there were no problems with safety, and no effect on infant weight or survival [135, 136].

Moderna's mRNA-1273 is a nucleoside-modRNA-based vaccine in an LNP formulation encoding the stabilizing S protein by replacing two prolines (S-2P, at 86 and 987). The structural rearrangement of the fusion S2 subunit is prevented in heptad repeat 1 located at the top of the S-2P. From March 2020, mRNA-1273 showed strongly biased expression of Th1 cytokines in people aged 18-71 years through a phase 1 clinical trial and a rapid S-2P antibody binding reaction (NCT04283461) [137, 138]. The FDA approved EUA for the COVID-19 pandemic in December 2020, validating the safety and efficacy of 94.1% at preventing COVID-19 through a 2-part phase 3 clinical trial (NCT04470427) [139]. In addition, mRNA-1273 showed antibody activity for all ages for 180 days after the second dose (209 days) through the RBD ELISA and Neutralization assay [140].

After the outbreak of the Omicron (B.1.1.529) mutation in November 2021, the fourth vaccination became inevitable despite receiving the second and booster vaccinations. In an open label, non-randomized clinical study, mRNA-1273 showed 9.73-fold the IgG titer and 7.23-fold the neutralizing titer in the participants receiving fourth dose vaccination compared to the participants who 5 months after the booster vaccination aged 18 years and older (NCT NCT05230953). Also, BNT162b2 showed 7.01-fold the IgG titer and 10.73-fold the neutralizing titer in the participants receiving fourth dose vaccination (NCT05231005) [141].

LNPs in vaccines against mRNA COVID-19 are similar to four major components, although the molar lipid composition differs [5, 113]. Because the mRNA-LNPs of both companies have the anionic property of mRNA, ionizable lipids (Pfizer (ALC-0315); Moderna (SM-102)), which are positively charged (protonation) at low pH, are used to construct the LNPs. The phospholipid, 1-2-distearoy-sn-glycero-3-phosphocholine (DSPC), and cholesterol are helper lipids that can improve the stability, tolerability, and biodistribution. PEGylated lipids (Pfizer, ALC-0159 (PEG-DMA); Moderna (1,2-dimyristoyl-rac-glycero-3 methoxypolyethylene glycol-2000) (PEG-DMG)) increase the enhanced permeability and retention (EPR) effect to ensure stability and prevent aggregation during storage [20, 131] as seen in Table 4.

In the mRNA part, to prevent degradation and stabilize the mRNA structure, 1-methyl-pseudouridine (m1Ѱ), one of the naturally occurring converted uridines, in modRNA was combined to induce secondary structure changes in the mRNA to correlate with high protein translation. Another third mRNA candidate vaccine [19, 131], CvnCov from CureVAC AG, did not meet the FDA approval criteria with an overall efficacy of 48% in the 2b / 3 clinical trial (NCT04652102) between December 11, 2020 and April 12, 2021 [142-144]. It has been suggested that one of the reasons was that, unlike the Pfizer-BioNTech or Moderna vaccine, it does not contain m1Ѱ.

Local events such as pain at the injection site, edema, erythema, or systemic events such as fever, headache, vomit, and chills are commonly reported after vaccination against COVID-19. Specifically, on May 17, 2022 for BNT162b2 or on March 29, 2022 for mRNA-1273, the FDA revised the Patient and Provider Fact Sheet because severe systemic outbreaks of anaphylaxis, thrombosis, and myocarditis were reported as COVID-19 vaccination expanded worldwide. As of March 14, 2022, the Vaccine Adverse Event Report System (www.vaers.hhs.gov, VAERS) has received 4,626 (2,757 for BNT162b2, 1,869 for mRNA-1273) reports of myocarditis or pericarditis among people 3 years of age or older who have received the both COVID-19 vaccine. In addition, 11,997 (9,211 for BNT162b2, 2,786 for mRNA-1273) cases reported by European Union/European Economic Area (EU/EEA) EudraVigilance system (https://www.ema.europa.eu/) [145]. Most have been reported after vaccination with the mRNA COVID-19 vaccine (Pfizer-BioNTech or Moderna), especially in male adolescents and young adults, but there is an increasing trend in females as well [146-149]. Although the correlation between mRNA-LNP-based vaccines against COVID-19 and myocarditis has not yet been clearly elucidated, the strongest hypothesis is that cationic lipids in the LNP component induce antibody-mediated cytokine expression and activate aberrant apoptosis [106, 150]. Moreover, among the lipid components, PEGylated lipids can activate the host immune response and stimulate the complement system to induce hypersensitivity reactions after systemic or local administration. Due to these stability problems, studies that can replace PEG are needed and are in progress [20].

Recently, rapid and useful vaccines have been developed against COVID-19, but many mutant variants are emerging [151]. To date, the five representative variants known are Alpha (B.1.1.7), Beta (B.1.351), Gamma (P.1), Delta (B.1.617.2) and Omicron (B.1.1.529) which are the forms of the receptor binding domain (RBD) in the S protein [152-156]. If its protein continues to mutate due to the change of the spike gene, angiotensin-converting enzyme 2 (ACE2), the binding to the major receptor, is impaired [157]. These changes alter infection and mortality rates and reduce the efficacy of vaccines being developed based on the original COVID-19 strain. The effects and efficacy against the COVID-19 mutant using BNT162b2 (Pfizer/BioNTech) and mRNA-1273 (Moderna), mRNA-LNP vaccines that have passed FDA approval [157], are summarized in Table 5.

Cancer LNP-based mRNA therapeutics vaccines and therapeutics

mRNA vaccines promote specific immune responses while encoding antigens which can be presented to antigen-presenting cells (APCs) [19]. These antigens regulate the immune response against a tumor through two T-cell responses. One antigen presented by major histocompatibility complex (MHC) class 1 makes an immune response with CD8+ T cells. Another antigen released by lysosomes presented by MHC class 2 induces an immune response with CD4+ T cells [158, 159].

Cancer vaccines have a dual role, functioning as both a prophylactic and therapeutic. The mutations of tumor cells during carcinogenesis produce modified proteins called neoantigens. Utilizing neoantigens can produce customized/personalized neoepitopes for cancer vaccines to improve the anti-tumor immune responses compared to conventional cancer vaccines as shown in Table 6 [160].

BNT111, IVAC MUTANOME (FixVAC), from BioNTech RNA Pharmaceuticals GmbH's is a poly neoantigen encoding RNA vaccine that targets unique mutational features in individual patients. From December 2013 to February 2017, a poly neoantigen immune response to the vaccine antigen was detected in all patients, and 60% of the 125 selected neonatal epitopes induced CD8+ and CD4+ T cell responses in malignant melanoma patients aged 18-49 years. (NCT02035956). Next, FixVac (BNT111), a Lipo-Mutanome Engineered RNA Immuno-Therapy (Lipo-MERIT), based on a nanoparticulate liposomal RNA (RNA-LPX) formulation, is a mRNA vaccine encoding four non-mutated antigens, also called tumor-associated antigens (TAAs), and has undergone a phase 1 clinical trial in patients with advanced melanoma. Most patients showed recruitment of the potent CD4+ and CD8+ T-cell immunity to antigens and a synergistic event with the combination of FixVac and anti-programmed death 1 (PD-1) in patients with experience with checkpoint inhibitors, demonstrating that TAAs may be useful as cancer vaccine targets (NCT02410733) [8]. Based on a previous phase 1 clinical trial, the phase 2 clinical trial of BNT111 which in combination with Libtayo (Cemiplimab) in patients with unresectable stage 3 or 4 melanoma was started on May 19, 2021 (NCT04526899).

From October 2016 to May 2020, BioNTech SE's TNBC-MERIT was being conducted in 42 triple-negative breast cancer (TNBC) patients over the age of 18 years in a phase 1 clinical trial. The group treated with a combination of the IVAC_WAREHOUSE_bre1_uID and IVAC_MUTANOME_uID vaccine showed a strong induction of CD8+ T cells (NCT02316457) [108, 161].

Because neoantigens generated by somatic changes in cancer cells are very different between individual patients, it is necessary to develop a personalized vaccine. Moderna developed mRNA-4157, a mRNA encoding 43 neoantigens, and conducted phase 1 clinical trials on 142 solid cancer patients over the age of 18 years since August 2017. They divided patients with a resected solid cancer treated with mRNA alone and patients with an unresectable solid cancer or melanoma treated with pembrolizumab in combination into four groups. The median progression survival was longer in the group with the combination therapy (9.8 months) than in the group with the monotherapy (8 months) (NCT03313778). After entering the phase 2 clinical trial from January 2019, 150 patients aged 18 years and older were evaluated with mRNA-4157 and pembrolizumab as a postoperative adjuvant therapy that improves recurrence free survival compared to pembrolizumab only in patients with a high risk of recurrence of completely resected melanoma (NCT03897881). Similarly, in May 2018, there was also a first clinical trial using mRNA-4650, which encodes 20 neoantigens from 4 gastrointestinal cancer patients. Although a clinical response could not be obtained through a phase ½ clinical trial, it was able to elicit a response from CD4+ T cells (NCT03480152) [108, 162].

Instead of vaccination, clinical trials using mRNA-LNP drugs that encode co-stimulator molecules that enhance T-cell activity in the pro-inflammatory phase or deliver cytokines are also underway. mRNA-2416 is an OX40L (ligand of OX40)-encoding mRNA-LNP therapeutic. In August 2017, based on the results of the evaluation of antitumor efficacy in syngeneic colon and ovarian carcinoma tumor models in MC38-S and ID8 mice, a clinical phase ½ trial was conducted for the OX40L-encoding mRNA-LNP treatment of 117 patients over the age of 18 years with a solid tumor or lymphoma. This is a human first, phase 1, dose escalation (1 to 8 mg) clinical study, and the study was designed to determine the safety and efficacy of repeated intratumorally injections of mRNA-2416 alone and intravenous injection of a combination with durvalumab for patients. It was confirmed that the response of OX40L and T cells was increased at the injection site in the tumor (NCT03323398) [108].

As another mRNA-LNP treatment, mRNA-2752 encoding OX40L, pro-inflammatory cytokines, interleukin-23 (IL-23), and interleukin-36 gamma (IL-36γ) was injected 7 times for 2 weeks with dose escalation, followed by a combination therapy with durvalumab in 126 patients over the age of 18 years with a solid tumor or lymphoma. Both monotherapy and combination therapy of duravalumab have been shown to be associated with tumor shrinkage in lesions, and these data suggest sustained immunomodulatory effects of TNF-α, IFN-γ, and programmed death ligand 1 (PD-L1) with clinically low toxic levels in tumor and plasma assays (NCT03739931) [163].

Autogene cevemeran (RO7198457) is an mRNA vaccine designed to stimulate T-cell responses against neoantigens with iNeST's Lipo-MERIT. From December 2017 until now, the phase 1a / 1b clinical trial has been conducted with 25 to 100 ug of RO7198457 as a single therapy or in combination with 1200 mg of anti-PD-L1, Atezolizumab, being given to patients of melanoma, NSCLC, TNBC, colon cancer, and bladder cancer. In phase 1a, in the peripheral blood of 14 out of 16 patients (87%), T cell responses against RO7187457-induced neoantigens were observed by ex vivo ELISPOT or MHC multimer assays. In addition, it showed the activity of an innate immunity inducer because pro-inflammatory cytokines were released according to each dose. In the 1b clinical trial, 142 patients with various solid tumors were treated once every 3 weeks (Q3W) while increasing the dose of RO7198457 from 3 doses at 25 μg to 50 μg while fixing the dose of atezolizumab to 1200 mg. In TNBC patients, more than 5% of the CD8 T scale was induced in the peripheral blood, and there was mainly an effector memory phenotype and high expression of CD8+PD-1 of 99.2% (NCT03289962) [164].

Utilization of in vivo imaging for development of LNP-based RNA therapeutics

The major challenge of in vivo delivery of RNA vaccines and therapeutics is that RNA molecules are highly unstable to physiological conditions due to ubiquitous RNases and are quickly cleared following systemic circulation. Therefore, LNPs are used as the RNA delivery system, protecting RNA from degradation and showing a longer circulation half-time than naked RNA [165]. LNPs are also used to facilitate intracellular uptake (endocytosis), endosomal escape, and reduce undesired immunotoxicity [166, 167]. Given the advantages of RNA delivery research using LNP, the PK and PD profiles are important biopharmaceutical aspects after LNP administration.

Figure 6A-E provides an overview of the main routes for LNP-based therapeutics administration which are subcutaneous (SC), intramuscular (IM), intravenous (IV), intradermal (ID), and oral. LNPs are usually injected through a systemic route: enteral and parental routes [168]. IM injection, a parental route, is especially used as an RNA vaccine for infectious diseases and cancer. Recently, COVID-19 mRNA-LNP vaccines from Moderna and Pfizer/BioNTech have also been intramuscularly administered into the deltoid muscle. In particular, both mRNA-LNP vaccines have more than a 90% vaccine efficacy when inoculated twice with IM injection at a 3-4 week interval [130, 132]. Continuously producing proteins in muscle cells is an advantage in effective nucleic acid-based vaccines administered by IM injection because muscles have abundant blood vessels. It can recruit various immune cells to the injection site, facilitate protein expression, and trigger the immune system [169]. Generally, an IV administered LNP is deposited in the liver primarily; therefore, liver targeted LNP-based RNA therapeutics would prefer the IV administration. For example, Patisiran, an FDA approved LNP-based siRNA therapeutics, is administered through the vein because its target is hepatocyte produced transthyretin amyloid [170]. Additionally, IV injection is used to treat genetic disorders [5].

In vivo imaging has played an increasing role in the process of drug development. In vivo imaging has roles in accelerating the drug development process by the identification of drug targets, evaluation of the pharmacokinetics and pharmacodynamics of the drugs, and selection of optimal candidates [9, 10]. Also, in vivo imaging can be used to develop companion imaging biomarkers which can facilitate patient selection for clinical trials. Furthermore, the imaging biomarkers that were developed for the clinical trials, can be utilized as predictive biomarkers in clinic as shown in Figure 7 [9, 10, 171]. Currently, in vivo imaging techniques is under-utilized in the process of development of LNP-based RNA Therapeutics. In this chapter, in vivo imaging techniques in the development of LNP-based RNA therapeutics will be summarized (Table 7) and describe areas that require future research.

PD analysis using imaging LNP

By the direct gene expression modulation ability of RNA therapeutics, PD can be easily evaluated by imaging. A fluorescent protein coding mRNA used for imaging can be used to assess the PD of the LNP for mRNA therapeutics. As a reporter gene formulated in LNPs, luciferase mRNA is effectively delivered to certain tissues or organs by avoiding metabolic enzymes by LNPs and is translated as a luminescent protein that can be visible using an IVIS (In Vivo Imaging System) [172, 173]. Kim et al. utilized fluorescence in vivo imaging to show that different types of ionizable lipids have different in vivo efficacies in LNP formulations using LNPs loaded with luciferase genes [174] as shown in Figure 8A. In vivo imaging can elucidate different profiles of protein expression according to the administration routes. Pardi et al. compared the expression levels of firefly luciferase mRNA-LNPs administered at a dose of 0.005-0.250 mg/kg with six different injection routes [IV, intraperitoneal (IP), IM, SC, ID, and intratracheal (IT)]. The levels of protein translation were measured using in vivo imaging. Among the six groups, the IV administered groups showed the highest level of protein production. Meanwhile, the IM and ID injected groups showed the longest period (up to 10 days) of protein translation [21]. Additionally, in the case of siRNA, gene silencing can be imaged in vivo. Tao et al. developed a mouse model with liver-specific expression of a luciferase gene, and a luciferase siRNA-loaded LNP was injected to assess the silencing effect of the siRNA therapeutics [175]. In addition, genomic editing can be imaged using special cell lines. Farbiak et al. reported that dendrimer-based lipid nanoparticles (dLNPs) encapsulating three nucleic acids (Cas9 mRNA, sgRNA, and ssDNA) can edit the gene of BFP/GFP switchable HEK293 cells, and thus, the gene editing efficiency can be evaluated by fluorescence imaging in vitro and in vivo [176] shown in Figure 8B. In vivo imaging is a powerful tool to demonstrate the PD of LNP-based RNA therapeutics. However, they can elicit the pharmacological effect through multiple steps, which are delivered to the target tissue by endocytosis to the target cells, endosomal escape, and translation. Therefore, if the imaging showed a negative result, then it is hard to pinpoint which process was not efficient. In that sense, a separate evaluation of each step will facilitate the process of developing efficient LNP-based RNA therapeutics.

 Figure 6 

Main systemic delivery routes of RNA-LNPs. The selection of an appropriate route of administration may affect the efficacy of RNA medicines. RNA-LNPs are generally administered by systemic injections: (A) intramuscular (IM), (B) subcutaneous (SC), (C) intradermal (ID), (D) intravenous (IV), and (E) oral route. Created with BioRender.com.

 Figure 7 

Potential role of imaging in development of LNP-based RNA therapeutics.

 Figure 8 

In vivo imaging of pharmacodynamics (PD) of LNP-based RNA therapeutics. (A) In vivo imaging was utilized to demonstrate luciferase gene expression, adapted from [174], and (B) gene editing efficacy, adapted from [176].

Moreover, for vaccines, the appropriate adaptive immune response is the most important aspect for their efficacy. mRNA-LNP vaccines can cause a prominent inflammatory response and induce a robust humoral response. LNPs can interact with pattern recognition receptors (PRRs) on antigen-presenting cells (APCs) and enhance pro-inflammatory cytokine release [177]. Additionally, Ndeupen et al. reported that robust neutrophil infiltration was found in muscle tissue 24 hours after intramuscular injection of the LNP [178]. This inflammatory response is considered as the causes for the side effect of vaccines and possibly reduce the efficacy to induce the adaptive immunity [179]. Zhang et al. reported that an anti-inflammatory (dexamethasone incorporated) luciferase mRNA-loaded LNP showed improved luciferase protein expression compared to conventional LNPs [179]. Therefore, careful assessment of the immune response by LNPs should be conducted during the development of LNP-based platforms [178, 180]. Currently, tissue samples are used to evaluate the inflammatory process after administration of LNP-based platforms. However, there are various in vivo imaging modalities to non-invasively evaluate the inflammatory process [181]. For example, ¹⁸F-fluorodexoyglucose PET can detect immune cells with increased metabolism, and is used clinically for the diagnosis of cardiac sarcoidosis and the differential diagnosis of fever of unknown origin (FUO) [182]. Translocator protein (TSPO) tracers are also available for inflammation PET imaging. In particular, TSPO can be used for imaging neuroinflammation because TSPO is overexpressed in activated microglias [183]. In vivo imaging has advantages in the assessment of the inflammatory process in the development of LNP-based RNA therapeutics because it is non-invasive and can be performed at multiple time points. Currently, inflammation imaging is not used for the development of LNP-based mRNA therapeutics, but it may facilitate the process of developing LNP-based mRNA therapeutics.

PK analysis using in vivo imaging of LNP

In vivo imaging can be used for PK evaluation of LNPs. In vivo imaging can be done by labeling a contrast agent in the LNP or mRNA [174]. The contrast agent can be iron oxide nanoparticles for magnetic resonance imaging, radionuclides for nuclear medicine imaging, an iodine agent for x-ray or CT imaging, or a fluorescence or luminescence dye for optical imaging. Fluorescent dyes are used most frequently in PK assessment of RNA therapeutics. Shi et al. reported that Cy5-labeled siRNA encapsulated LNP can be imaged in vivo to assess the biodistribution of the therapeutics. The siRNA showed high accumulation in the liver, spleen, and kidneys [184].

Among the various imaging methods, radionuclide imaging has the advantage to precisely assess the PK of drugs because of its high imaging sensitivity, and quantifiability [185]. Although multiple studies have utilized radionuclide imaging techniques to evaluate the PK of LNP therapeutics encapsulating conventional agents, there are few papers that assess the PK of LNP encapsulated RNAs [186]. Various radiolabeling methods of LNPs can be utilized to assess the PK of LNP-based RNA therapeutics [187]. These methods include surface radiolabeling and intraliposomal labeling. For surface radiolabeling, radionuclides either with or without chelators can be attached to the membrane or incorporated into the lipid bilayer. On the other hand, radionuclides can be encapsulated within the hydrophilic core using ionophores, or radioactive compounds can be trapped after passive diffusion into the hydrophilic core [187]. Radiolabeled LNPs can be used as a companion diagnostic for drug-loaded LNPs. Lee et al. developed a ⁶⁴Cu labeled liposome for in vivo imaging companion diagnostics for another liposomal drug. They showed that a high accumulation of the ⁶⁴Cu labeled liposome can predict a greater anti-tumor activity of other liposomal drugs shown in Figure 9 [188]. Although LNP encapsulating RNAs have a more complicated process to elicit a therapeutic effect than conventional liposomal drugs, the first step to achieve this goal will be the appropriate PK and that can be evaluated by in vivo imaging techniques. However, nucleic acid therapeutics can be damaged by ionizing radiation [189], and the integrity of RNA therapeutics using radionuclides for imaging should be analyzed before utilizing radionuclides in the PK evaluation of LNP-based RNA therapeutics.

 Figure 9 

In vivo companion diagnostics using a radiolabeled liposome. (A) MM-DX-929 a companion diagnostic agent which is highly PEGylated untargeted liposome encapsulating ⁶⁶Cu complexed with 4-DEAP-ATSC chelator. (B) Tumor volume change was significantly higher in tumor bearing mice with high deposition of MM-DX-929 compared to low deposition of the tracer. (C) Representative PET imaging of MM-DX-929 in tumor bearing mouse. (D) Axial PET/CT image shows different degrees of tumor MM-DX-929 uptakes, adapted from [188].

Endosomal escape analysis using the imaging of LNPs

Endosomal escape is a crucial step for the efficiency of LNP-based RNA therapeutics. Nanoparticles including LNPs enter cells through endocytic pathway in most cases. Endocytic vesicles undergo unidirectional process which includes fusion with early endosomes, maturation into late endosomes, and fusion with lysosomes [190, 191]. Lysosomes contain about 50 types of enzymes that can hydrolyze proteins, peptides, nucleic acids, lipids and polysaccharides [192]. Therefore, LNP-based RNA therapeutics delivered to the cells should escape from endosomes to elicit its therapeutics effect. However, there is no established method to evaluate endosomal escape in vivo. Currently, there are several methods to detect in vitro endosomal escape. The methods are fluorescent labeling assays, leakage assays, membrane lysis assays, and transfection assays [193]. The endosomal escape of fluorescent dye-labeled LNPs can be assessed by observation of the fluorescence signal pattern in the cells: a diffused pattern indicates endosomal escape while a punctate pattern implies the LNPs are still trapped [194]. This method is not quantitative, and inter-rater agreement could be low. Leakage assays utilize small fluorescent molecules such as calcein. The fluorescence signal of calcein is quenched in endosomes/lysosomes due to the low pH and high local concentration of the dye, and when endosomal escape occurs, a diffuse fluorescence signal can be seen in the cytoplasm [195]. Imaging membrane damage-associated markers can be done to evaluate endosomal escape. Rietz et al. reported that galectic-9 is a reliable marker for membrane damage and endosomal escape [196]. However, this method can only be used in genetically engineered cells or in fixed cells shown in Figure 10. Because all currently reported studies evaluating endosomal escape are limited to in vitro applications, the development of in vivo methods to assess the endosomal escape of LNPs is required to facilitate the development of LNP-based RNA therapeutics.

 Figure 10 

In vitro methods to assess the efficiency of endosomal escape. (A) Calcein leakage assay, adapted from [193]. (B) Confocal images of HeLa cells stained for galectin-3 after treatment of various small molecules. (C) HeLa cells expressing YFP-galectin-9 after treatment with chloroquine, which can facilitate endosomal escape. Adapted from [196].

Conclusion

With the rapid and successful development of LNP-based mRNA vaccines against COVID-19, LNP-based mRNA therapeutics are considered one of the most promising therapeutic platforms. The PK and PD of drugs have a major impact on the efficacy and safety of the drugs. Currently, imaging of gene expression changes using fluorescent genes is frequently used to jointly evaluate the PK and PD of LNP-based mRNA therapeutics. However, because this method reflects the results of all the steps at once, it is difficult to use for RNA therapeutics to optimize each step to induce activity. In vivo imaging of LNP-based RNA therapeutics containing contrast agents could be utilized to optimize the biodistribution of the candidate LNP and to predict the therapeutic efficacy of the LNP. Endosomal escape is a crucial step for LNP-based RNA therapeutics, but an in vivo imaging method to evaluate endosomal escape is currently lacking. Therefore, it is warranted to develop appropriate in vivo imaging methods to evaluate the PK and endosomal escape to facilitate the successful development of LNP-based RNA therapeutics.

Acknowledgements

This research was supported by grants funded by the National Research Foundation of Korea (NRF) (NRF-2019M2D2A1A01058210, NRF-2020R1C1C1009000, 2021M2E8A1039564), Creative-Pioneering Researchers Program through Seoul National University (SNU), Korea Evaluation Institute of Industrial Technology (KEIT) grant funded by the Korea government (MOTIE) (No. 20018522), and grants from Korean Government (22213MFDS421 from Ministry of Food and Drug Safety in 2022; NRF-2020R1A2C2011695 from Ministry of Science and ICT). Schematic illustrations were created with BioRender.

Competing Interests

Hyung-Jun Im is a consultant of Cellbion. Hyung-Jun Im is a co-founder and Chief Scientific Officer of Portrai. Hyewon Youn is a co-founder and Chief Scientific Officer of BIK-Therapeutics. There is no competing financial interest.

References

1. Sahin U, Karikó K, Türeci Ö. mRNA-based therapeutics—developing a new class of drugs. Nat Rev Drug Discov. 2014;13:759-80

2. Ostro MJ, Giacomoni D, Lavelle DON, Paxton W, Dray S. Evidence for translation of rabbit globin mRNA after liposomemediated insertion into a human cell line. Nature. 1978;274:921-3

3. Malone RW, Felgner PL, Verma IM. Cationic liposome-mediated RNA transfection. Proc Natl Acad Sci U S A. 1989;86:6077-81

4. Fenton OS, Kauffman KJ, McClellan RL, Appel EA, Dorkin JR, Tibbitt MW. et al. Bioinspired alkenyl amino alcohol ionizable lipid materials for highly potent in vivo mRNA delivery. Adv Mater. 2016;28:2939-43

5. Hou X, Zaks T, Langer R, Dong Y. Lipid nanoparticles for mRNA delivery. Nat Rev Mater. 2021

6. Jackson NAC, Kester KE, Casimiro D, Gurunathan S, DeRosa F. The promise of mRNA vaccines: a biotech and industrial perspective. NPJ Vaccines. 2020;5:11

7. Nanomedicine and the COVID-19 vaccines. Nat Nanotechnol. 2020; 15: 963.

8. Sahin U, Oehm P, Derhovanessian E, Jabulowsky RA, Vormehr M, Gold M. et al. An RNA vaccine drives immunity in checkpoint-inhibitor-treated melanoma. Nature. 2020;585:107-12

9. Lindner JR, Link J. Molecular Imaging in Drug Discovery and Development. Circ Cardiovasc Imaging. 2018;11:e005355

10. Willmann JK, van Bruggen N, Dinkelborg LM, Gambhir SS. Molecular imaging in drug development. Nat Rev Drug Discov. 2008;7:591-607

11. Smith BR, Gambhir SS. Nanomaterials for In Vivo Imaging. Chem Rev. 2017;117:901-86

12. Herrmann K, Schwaiger M, Lewis JS, Solomon SB, McNeil BJ, Baumann M. et al. Radiotheranostics: a roadmap for future development. Lancet Oncol. 2020;21:e146-e56

13. Lammers T, Aime S, Hennink WE, Storm G, Kiessling F. Theranostic Nanomedicine. Acc Chem Res. 2011;44:1029-38

14. Muthu MS, Leong DT, Mei L, Feng S-S. Nanotheranostics ˗ Application and Further Development of Nanomedicine Strategies for Advanced Theranostics. Theranostics. 2014;4:660-77

15. Malone RW, Felgner PL, Verma IM. Cationic liposome-mediated RNA transfection. Proceedings of the National Academy of Sciences. 1989;86:6077-81

16. Langer R, Folkman J. Polymers for the sustained release of proteins and other macromolecules. Nature. 1976;263:797-800

17. Dimitriadis GJ. Translation of rabbit globin mRNA introduced by liposomes into mouse lymphocytes. Nature. 1978;274:923-4

18. Liang Y, Huang L, Liu T. Development and Delivery Systems of mRNA Vaccines. Front Bioeng Biotechnol. 2021 9

19. Pardi N, Hogan MJ, Porter FW, Weissman D. mRNA vaccines—a new era in vaccinology. Nat Rev Drug Discov. 2018;17:261-79

20. Schoenmaker L, Witzigmann D, Kulkarni JA, Verbeke R, Kersten G, Jiskoot W. et al. mRNA-lipid nanoparticle COVID-19 vaccines: Structure and stability. Int J Pharm. 2021;601:120586

21. Pardi N, Tuyishime S, Muramatsu H, Kariko K, Mui BL, Tam YK. et al. Expression kinetics of nucleoside-modified mRNA delivered in lipid nanoparticles to mice by various routes. J Control Release. 2015;217:345-51

22. Samaridou E, Heyes J, Lutwyche P. Lipid nanoparticles for nucleic acid delivery: Current perspectives. Adv Drug Deliv Rev. 2020;154-155:37-63

23. Evers MJW, Kulkarni JA, van der Meel R, Cullis PR, Vader P, Schiffelers RM. State-of-the-Art Design and Rapid-Mixing Production Techniques of Lipid Nanoparticles for Nucleic Acid Delivery. Small Methods. 2018;2:1700375

24. Vallazza B, Petri S, Poleganov MA, Eberle F, Kuhn AN, Sahin U. Recombinant messenger RNA technology and its application in cancer immunotherapy, transcript replacement therapies, pluripotent stem cell induction, and beyond. Wiley Interdiscip Rev RNA. 2015;6:471-99

25. Hajj KA, Whitehead KA. Tools for translation: non-viral materials for therapeutic mRNA delivery. Nat Rev Mater. 2017;2:1-17

26. Kowalski PS, Rudra A, Miao L, Anderson DG. Delivering the messenger: advances in technologies for therapeutic mRNA delivery. Mol Ther. 2019;27:710-28

27. Meng C, Chen Z, Li G, Welte T, Shen H. Nanoplatforms for mRNA Therapeutics. Adv Ther (Weinh). 2021;4:2000099

28. Chonn A, Semple SC, Cullis PR. β2-Glycoprotein I Is a Major Protein Associated with Very Rapidly Cleared Liposomes in Vivo, Suggesting a Significant Role in the Immune Clearance of “Non-self” Particles (∗). J Biol Chem. 1995;270:25845-9

29. Schlich M, Palomba R, Costabile G, Mizrahy S, Pannuzzo M, Peer D. et al. Cytosolic delivery of nucleic acids: The case of ionizable lipid nanoparticles. Bioeng Transl Med. 2021;6:e10213

30. Gilleron J, Querbes W, Zeigerer A, Borodovsky A, Marsico G, Schubert U. et al. Image-based analysis of lipid nanoparticle-mediated siRNA delivery, intracellular trafficking and endosomal escape. Nat Biotechnol. 2013;31:638-46

31. Wittrup A, Ai A, Liu X, Hamar P, Trifonova R, Charisse K. et al. Visualizing lipid-formulated siRNA release from endosomes and target gene knockdown. Nat Biotechnol. 2015;33:870-6

32. Verbeke R, Lentacker I, De Smedt SC, Dewitte H. Three decades of messenger RNA vaccine development. Nano Today. 2019;28:100766

33. Kim J, Eygeris Y, Gupta M, Sahay G. Self-assembled mRNA vaccines. Adv Drug Deliv Rev. 2021;170:83-112

34. Reichmuth AM, Oberli MA, Jaklenec A, Langer R, Blankschtein D. mRNA vaccine delivery using lipid nanoparticles. Ther Deliv. 2016;7:319-34

35. Cheng X, Lee RJ. The role of helper lipids in lipid nanoparticles (LNPs) designed for oligonucleotide delivery. Adv Drug Deliv Rev. 2016;99:129-37

36. Zhang Y, Sun C, Wang C, Jankovic KE, Dong Y. Lipids and Lipid Derivatives for RNA Delivery. Chem Rev. 2021;121:12181-277

37. Eygeris Y, Gupta M, Kim J, Sahay G. Chemistry of Lipid Nanoparticles for RNA Delivery. Acc Chem Res. 2022;55:2-12

38. Aldosari B, Alfagih I, Almurshedi A. Lipid Nanoparticles as Delivery Systems for RNA-Based Vaccines. Pharmaceutics. 2021 p. 206

39. Koltover I, Salditt T, Rädler JO, Safinya CR. An inverted hexagonal phase of cationic liposome-DNA complexes related to DNA release and delivery. Science. 1998;281:78-81

40. Thewalt JL, Bloom M. Phosphatidylcholine: cholesterol phase diagrams. Biophys J. 1992;63:1176-81

41. Leung AK, Hafez IM, Baoukina S, Belliveau NM, Zhigaltsev IV, Afshinmanesh E. et al. Lipid Nanoparticles Containing siRNA Synthesized by Microfluidic Mixing Exhibit an Electron-Dense Nanostructured Core. J Phys Chem C Nanomater Interfaces. 2012;116:18440-50

42. Kanasty R, Dorkin JR, Vegas A, Anderson D. Delivery materials for siRNA therapeutics. Nat Mater. 2013;12:967-77

43. Fasbender A, Marshall J, Moninger TO, Grunst T, Cheng S, Welsh MJ. Effect of co-lipids in enhancing cationic lipid-mediated gene transfer in vitro and in vivo. Gene Ther. 1997;4:716-25

44. Farhood H, Serbina N, Huang L. The role of dioleoyl phosphatidylethanolamine in cationic liposome mediated gene transfer. Biochim Biophys Acta Biomembr. 1995;1235:289-95

45. Mok KW, Lam AM, Cullis PR. Stabilized plasmid-lipid particles: factors influencing plasmid entrapment and transfection properties. Biochim Biophys Acta. 1999;1419:137-50

46. Bieong-Kil K, Kyung-Oh D, Guen-Bae H. Transfection Property of a New Cholesterol-Based Cationic Lipid Containing Tri-2-Hydroxyethylamine as Gene Delivery Vehicle. J Microbiol Biotechnol. 2012;22:866-71

47. Patel S, Ashwanikumar N, Robinson E, Xia Y, Mihai C, Griffith JP. et al. Naturally-occurring cholesterol analogues in lipid nanoparticles induce polymorphic shape and enhance intracellular delivery of mRNA. Nat Commun. 2020;11:1-13

48. Kotouček J, Hubatka F, Mašek J, Kulich P, Velínská K, Bezděková J. et al. Preparation of nanoliposomes by microfluidic mixing in herring-bone channel and the role of membrane fluidity in liposomes formation. Sci Rep. 2020;10:5595

49. Knop K, Hoogenboom R, Fischer D, Schubert US. Poly (ethylene glycol) in drug delivery: pros and cons as well as potential alternatives. Angew Chem Int Ed Engl. 2010;49:6288-308

50. Ryals RC, Patel S, Acosta C, McKinney M, Pennesi ME, Sahay G. The effects of PEGylation on LNP based mRNA delivery to the eye. Plos one. 2020;15:e0241006

51. Akinc A, Goldberg M, Qin J, Dorkin JR, Gamba-Vitalo C, Maier M. et al. Development of lipidoid-siRNA formulations for systemic delivery to the liver. Mol Ther. 2009;17:872-9

52. Zhu X, Tao W, Liu D, Wu J, Guo Z, Ji X. et al. Surface De-PEGylation controls nanoparticle-mediated siRNA delivery in vitro and in vivo. Theranostics. 2017;7:1990

53. Allen TM. The use of glycolipids and hydrophilic polymers in avoiding rapid uptake of liposomes by the mononuclear phagocyte system. Adv Drug Deliv Rev. 1994;13:285-309

54. Bao Y, Jin Y, Chivukula P, Zhang J, Liu Y, Liu J. et al. Effect of PEGylation on biodistribution and gene silencing of siRNA/lipid nanoparticle complexes. Pharm Res. 2013;30:342-51

55. Chen S, Tam YY, Lin PJ, Leung AK, Tam YK, Cullis PR. Development of lipid nanoparticle formulations of siRNA for hepatocyte gene silencing following subcutaneous administration. J Control Release. 2014;196:106-12

56. Witzigmann D, Kulkarni JA, Leung J, Chen S, Cullis PR, van der Meel R. Lipid nanoparticle technology for therapeutic gene regulation in the liver. Adv Drug Deliv Rev. 2020;159:344-63

57. Akinc A, Querbes W, De S, Qin J, Frank-Kamenetsky M, Jayaprakash KN. et al. Targeted delivery of RNAi therapeutics with endogenous and exogenous ligand-based mechanisms. Mol Ther. 2010;18:1357-64

58. Schöttler S, Becker G, Winzen S, Steinbach T, Mohr K, Landfester K. et al. Protein adsorption is required for stealth effect of poly(ethylene glycol)- and poly(phosphoester)-coated nanocarriers. Nat Nanotechnol. 2016;11:372-7

59. Maier MA, Jayaraman M, Matsuda S, Liu J, Barros S, Querbes W. et al. Biodegradable Lipids Enabling Rapidly Eliminated Lipid Nanoparticles for Systemic Delivery of RNAi Therapeutics. Mol Ther. 2013;21:1570-8

60. Webb MS, Saxon D, Wong FM, Lim HJ, Wang Z, Bally MB. et al. Comparison of different hydrophobic anchors conjugated to poly(ethylene glycol): effects on the pharmacokinetics of liposomal vincristine. Biochim Biophys Acta. 1998;1372:272-82

61. Ambegia E, Ansell S, Cullis P, Heyes J, Palmer L, MacLachlan I. Stabilized plasmid-lipid particles containing PEG-diacylglycerols exhibit extended circulation lifetimes and tumor selective gene expression. Biochim Biophys Acta. 2005;1669:155-63

62. Braeckmans K, Buyens K, Bouquet W, Vervaet C, Joye P, Vos FD. et al. Sizing Nanomatter in Biological Fluids by Fluorescence Single Particle Tracking. Nano Lett. 2010;10:4435-42

63. Shi F, Wasungu L, Nomden A, Stuart MCA, Polushkin E, Engberts JBFN. et al. Interference of poly(ethylene glycol)-lipid analogues with cationic-lipid-mediated delivery of oligonucleotides; role of lipid exchangeability and non-lamellar transitions. Biochem J. 2002;366:333-41

64. Ju Y, Lee WS, Pilkington EH, Kelly HG, Li S, Selva KJ. et al. Anti-PEG Antibodies Boosted in Humans by SARS-CoV-2 Lipid Nanoparticle mRNA Vaccine. ACS Nano. 2022;16:11769-80

65. Carreño JM, Singh G, Tcheou J, Srivastava K, Gleason C, Muramatsu H. et al. mRNA-1273 but not BNT162b2 induces antibodies against polyethylene glycol (PEG) contained in mRNA-based vaccine formulations. medRxiv. 2022. 2022 04.15.22273914

66. Sherman MR, Williams LD, Sobczyk MA, Michaels SJ, Saifer MGP. Role of the Methoxy Group in Immune Responses to mPEG-Protein Conjugates. Bioconjug Chem. 2012;23:485-99

67. Suzuki T, Suzuki Y, Hihara T, Kubara K, Kondo K, Hyodo K. et al. PEG shedding-rate-dependent blood clearance of PEGylated lipid nanoparticles in mice: Faster PEG shedding attenuates anti-PEG IgM production. Int J Pharm. 2020;588:119792

68. Chen B-M, Cheng T-L, Roffler SR. Polyethylene Glycol Immunogenicity: Theoretical, Clinical, and Practical Aspects of Anti-Polyethylene Glycol Antibodies. ACS Nano. 2021;15:14022-48

69. Szebeni J, Storm G, Ljubimova JY, Castells M, Phillips EJ, Turjeman K. et al. Applying lessons learned from nanomedicines to understand rare hypersensitivity reactions to mRNA-based SARS-CoV-2 vaccines. Nat Nanotechnol. 2022;17:337-46

70. Barba AA, Bochicchio S, Dalmoro A, Lamberti G. Lipid Delivery Systems for Nucleic-Acid-Based-Drugs: From Production to Clinical Applications. Pharmaceutics. 2019;11:360

71. Meure LA, Foster NR, Dehghani F. Conventional and dense gas techniques for the production of liposomes: a review. Aaps PharmSciTech. 2008;9:798-809

72. Crooke ST. Antisense Drug Technology: Principles, Strategies, and Applications. 2nd Edition ed. Boca Raton: CRC Press. 2007

73. Bangham AD, Horne RW. Negative staining of phospholipids and their structural modification by surface-active agents as observed in the electron microscope. J Mol Biol. 1964;8:660-IN10

74. Weissig V, Torchilin VP. Liposomes: a practical approach. In: Surface modifications of liposomes. Oxford University Press, Oxford. 1999

75. Angela Barba A, Lamberti G, Sardo C, Dapas B, Abrami M, Grassi M. et al. Novel lipid and polymeric materials as delivery systems for nucleic acid based drugs. Curr Drug Metab. 2015;16:427-52

76. Bochicchio S, Dalmoro A, Angela Barba A, Grassi G, Lamberti G. Liposomes as siRNA delivery vectors. Curr Drug Metab. 2014;15:882-92

77. Barba AA, Bochicchio S, Lamberti G, Dalmoro A. Ultrasonic energy in liposome production: process modelling and size calculation. Soft Matter. 2014;10:2574-81

78. Szoka Jr F, Papahadjopoulos D. Comparative properties and methods of preparation of lipid vesicles (liposomes). Annu Rev Biophys Bioeng. 1980;9:467-508

79. MacLachlan I. Liposomal formulations for nucleic acid delivery. Antisense Drug Technology: CRC press. 2007 p. 255-88

80. Wagner A, Vorauer-Uhl K. Liposome technology for industrial purposes. J Drug Deliv. 2011. 2011

81. Hood RR, DeVoe DL. High-Throughput Continuous Flow Production of Nanoscale Liposomes by Microfluidic Vertical Flow Focusing. Small. 2015;11:5790-9

82. Garg S, Heuck G, Ip S, Ramsay E. Microfluidics: a transformational tool for nanomedicine development and production. J Drug Target. 2016;24:821-35

83. Wagner A, Vorauer-Uhl K, Kreismayr G, Katinger H. THE CROSSFLOW INJECTION TECHNIQUE: AN IMPROVEMENT OF THE ETHANOL INJECTION METHOD. J Liposome Res. 2002;12:259-70

84. Gouda A, Sakr OS, Nasr M, Sammour O. Ethanol injection technique for liposomes formulation: An insight into development, influencing factors, challenges and applications. J Drug Deliv Sci Technol. 2021;61:102174

85. Batzri S, Korn ED. Single bilayer liposomes prepared without sonication. Biochim Biophys Acta Biomembr. 1973;298:1015-9

86. Buschmann MD, Carrasco MJ, Alishetty S, Paige M, Alameh MG, Weissman D. Nanomaterial Delivery Systems for mRNA Vaccines. Vaccines. 2021 9

87. Hauser HO. The effect of ultrasonic irradiation on the chemical structure of egg lecithin. Biochem Biophys Res Commun. 1971;45:1049-55

88. Koynova R, Tenchov B. Recent Progress in Liposome Production, Relevance to Drug Delivery and Nanomedicine. Recent Pat Nanotechnol. 2015;9:86-93

89. Valencia PM, Farokhzad OC, Karnik R, Langer R. Microfluidic technologies for accelerating the clinical translation of nanoparticles. Nature Nanotechnology. 2012;7:623-9

90. Hirota S, de Ilarduya CT, Barron LG, Szoka Jr FC. Simple mixing device to reproducibly prepare cationic lipid-DNA complexes (lipoplexes). Biotechniques. 1999;27:286-90

91. Davies LA, Nunez-Alonso GA, Hebel HL, Scheule RK, Cheng SH, Hyde SC. et al. A novel mixing device for the reproducible generation of nonviral gene therapy formulations. Biotechniques. 2010;49:666-8

92. Kulkarni JA, Darjuan MM, Mercer JE, Chen S, van der Meel R, Thewalt JL. et al. On the Formation and Morphology of Lipid Nanoparticles Containing Ionizable Cationic Lipids and siRNA. ACS Nano. 2018;12:4787-95

93. Kulkarni JA, Tam YYC, Chen S, Tam YK, Zaifman J, Cullis PR. et al. Rapid synthesis of lipid nanoparticles containing hydrophobic inorganic nanoparticles. Nanoscale. 2017;9:13600-9

94. Goswami R, Chatzikleanthous D, Lou G, Giusti F, Bonci A, Taccone M. et al. Mannosylation of LNP Results in Improved Potency for Self-Amplifying RNA (SAM) Vaccines. ACS Infect Dis. 2019;5:1546-58

95. Chen S, Zaifman J, Kulkarni JA, Zhigaltsev IV, Tam YK, Ciufolini MA. et al. Dexamethasone prodrugs as potent suppressors of the immunostimulatory effects of lipid nanoparticle formulations of nucleic acids. J Control Release. 2018;286:46-54

96. Lazzaro S, Giovani C, Mangiavacchi S, Magini D, Maione D, Baudner B. et al. CD8 T-cell priming upon mRNA vaccination is restricted to bone-marrow-derived antigen-presenting cells and may involve antigen transfer from myocytes. Immunology. 2015;146:312-26

97. Geall AJ, Verma A, Otten GR, Shaw CA, Hekele A, Banerjee K. et al. Nonviral delivery of self-amplifying RNA vaccines. Proc Natl Acad Sci U S A. 2012;109:14604-9

98. Andreussi T, Galletti C, Mauri R, Camarri S, Salvetti MV. Flow regimes in T-shaped micro-mixers. Comput Chem Eng. 2015;76:150-9

99. Stroock AD, Dertinger SKW, Ajdari A, Mezić I, Stone HA, Whitesides GM. Chaotic mixer for microchannels. Science. 2002;295:647-51

100. Zhigaltsev IV, Belliveau N, Hafez I, Leung AKK, Huft J, Hansen C. et al. Bottom-up design and synthesis of limit size lipid nanoparticle systems with aqueous and triglyceride cores using millisecond microfluidic mixing. Langmuir. 2012;28:3633-40

101. Cornebise M, Narayanan E, Xia Y, Acosta E, Ci L, Koch H. et al. Discovery of a Novel Amino Lipid That Improves Lipid Nanoparticle Performance through Specific Interactions with mRNA. Adv Funct Mater. 2022;32:2106727

102. Shepherd SJ, Warzecha CC, Yadavali S, El-Mayta R, Alameh M-G, Wang L. et al. Scalable mRNA and siRNA Lipid Nanoparticle Production Using a Parallelized Microfluidic Device. Nano Lett. 2021;21:5671-80

103. Belliveau NM, Huft J, Lin PJ, Chen S, Leung AK, Leaver TJ. et al. Microfluidic Synthesis of Highly Potent Limit-size Lipid Nanoparticles for In Vivo Delivery of siRNA. Mol Ther Nucleic Acids. 2012;1:e37

104. Allen L, Ansel HC. Ansel's pharmaceutical dosage forms and drug delivery systems: Lippincott Williams & Wilkins; 2013

105. Guimarães Sá Correia M, Briuglia ML, Niosi F, Lamprou DA. Microfluidic manufacturing of phospholipid nanoparticles: Stability, encapsulation efficacy, and drug release. Int J Pharm. 2017;516:91-9

106. Hassett KJ, Benenato KE, Jacquinet E, Lee A, Woods A, Yuzhakov O. et al. Optimization of Lipid Nanoparticles for Intramuscular Administration of mRNA Vaccines. Mol Ther Nucleic Acids. 2019;15:1-11

107. Hassett KJ, Higgins J, Woods A, Levy B, Xia Y, Hsiao CJ. et al. Impact of lipid nanoparticle size on mRNA vaccine immunogenicity. J Control Release. 2021;335:237-46

108. Miao L, Zhang Y, Huang L. mRNA vaccine for cancer immunotherapy. Mol Cancer. 2021;20:41

109. Balwani M, Sardh E, Ventura P, Peiró PA, Rees DC, Stölzel U. et al. Phase 3 Trial of RNAi Therapeutic Givosiran for Acute Intermittent Porphyria. N Engl J Med. 2020;382:2289-301

110. Agarwal S, Simon AR, Goel V, Habtemariam BA, Clausen VA, Kim JB. et al. Pharmacokinetics and Pharmacodynamics of the Small Interfering Ribonucleic Acid, Givosiran, in Patients With Acute Hepatic Porphyria. Clin Pharmacol Ther. 2020;108:63-72

111. Sahin U, Karikó K, Türeci Ö. mRNA-based therapeutics — developing a new class of drugs. Nature Reviews Drug Discovery. 2014;13:759-80

112. Gómez-Aguado I, Rodríguez-Castejón J, Vicente-Pascual M, Rodríguez-Gascón A, Solinís MÁ, Del Pozo-Rodríguez A. Nanomedicines to Deliver mRNA: State of the Art and Future Perspectives. Nanomaterials (Basel). 2020;10:364

113. Tenchov R, Bird R, Curtze AE, Zhou Q. Lipid Nanoparticles─From Liposomes to mRNA Vaccine Delivery, a Landscape of Research Diversity and Advancement. ACS Nano. 2021;15:16982-7015

114. Maruggi G, Zhang C, Li J, Ulmer JB, Yu D. mRNA as a Transformative Technology for Vaccine Development to Control Infectious Diseases. Mol Ther. 2019;27:757-72

115. Fuller DH, Berglund P. Amplifying RNA Vaccine Development. N Engl J Med. 2020;382:2469-71

116. Blakney AK, Ip S, Geall AJ. An Update on Self-Amplifying mRNA Vaccine Development. Vaccines (Basel). 2021 9

117. Wesselhoeft RA, Kowalski PS, Anderson DG. Engineering circular RNA for potent and stable translation in eukaryotic cells. Nat Commun. 2018;9:2629

118. Kristensen LS, Andersen MS, Stagsted LVW, Ebbesen KK, Hansen TB, Kjems J. The biogenesis, biology and characterization of circular RNAs. Nat Rev Genet. 2019;20:675-91

119. He AT, Liu J, Li F, Yang BB. Targeting circular RNAs as a therapeutic approach: current strategies and challenges. Signal Transduct Target Ther. 2021;6:185

120. Alberer M, Gnad-Vogt U, Hong HS, Mehr KT, Backert L, Finak G. et al. Safety and immunogenicity of a mRNA rabies vaccine in healthy adults: an open-label, non-randomised, prospective, first-in-human phase 1 clinical trial. Lancet. 2017;390:1511-20

121. Aldrich C, Leroux-Roels I, Huang KB, Bica MA, Loeliger E, Schoenborn-Kellenberger O. et al. Proof-of-concept of a low-dose unmodified mRNA-based rabies vaccine formulated with lipid nanoparticles in human volunteers: A phase 1 trial. Vaccine. 2021;39:1310-8

122. Bahl K, Senn JJ, Yuzhakov O, Bulychev A, Brito LA, Hassett KJ. et al. Preclinical and Clinical Demonstration of Immunogenicity by mRNA Vaccines against H10N8 and H7N9 Influenza Viruses. Mol Ther. 2017;25:1316-27

123. Feldman RA, Fuhr R, Smolenov I, Mick Ribeiro A, Panther L, Watson M. et al. mRNA vaccines against H10N8 and H7N9 influenza viruses of pandemic potential are immunogenic and well tolerated in healthy adults in phase 1 randomized clinical trials. Vaccine. 2019;37:3326-34

124. Richner JM, Jagger BW, Shan C, Fontes CR, Dowd KA, Cao B. et al. Vaccine Mediated Protection Against Zika Virus-Induced Congenital Disease. Cell. 2017;170:273-83.e12

125. Castanha PMS, Marques ETA. A Glimmer of Hope: Recent Updates and Future Challenges in Zika Vaccine Development. Viruses. 2020 12

126. Richner JM, Himansu S, Dowd KA, Butler SL, Salazar V, Fox JM. et al. Modified mRNA Vaccines Protect against Zika Virus Infection. Cell. 2017;168:1114-25.e10

127. Nelson CS, Jenks JA, Pardi N, Goodwin M, Roark H, Edwards W. et al. Human Cytomegalovirus Glycoprotein B Nucleoside-Modified mRNA Vaccine Elicits Antibody Responses with Greater Durability and Breadth than MF59-Adjuvanted gB Protein Immunization. J Virol. 2020 94

128. Scarpini S, Morigi F, Betti L, Dondi A, Biagi C, Lanari M. Development of a Vaccine against Human Cytomegalovirus: Advances, Barriers, and Implications for the Clinical Practice. Vaccines (Basel). 2021 9

129. Krammer F. SARS-CoV-2 vaccines in development. Nature. 2020;586:516-27

130. Zhu N, Zhang D, Wang W, Li X, Yang B, Song J. et al. A Novel Coronavirus from Patients with Pneumonia in China, 2019. N Engl J Med. 2020;382:727-33

131. Verbeke R, Lentacker I, De Smedt SC, Dewitte H. The dawn of mRNA vaccines: The COVID-19 case. J Control Release. 2021;333:511-20

132. Walsh EE, Frenck RW, Falsey AR, Kitchin N, Absalon J, Gurtman A. et al. Safety and Immunogenicity of Two RNA-Based Covid-19 Vaccine Candidates. N Engl J Med. 2020;383:2439-50

133. Thomas SJ, Moreira ED, Kitchin N, Absalon J, Gurtman A, Lockhart S. et al. Safety and Efficacy of the BNT162b2 mRNA Covid-19 Vaccine through 6 Months. N Engl J Med. 2021;385:1761-73

134. Frenck RW Jr, Klein NP, Kitchin N, Gurtman A, Absalon J, Lockhart S. et al. Safety, Immunogenicity, and Efficacy of the BNT162b2 Covid-19 Vaccine in Adolescents. N Engl J Med. 2021;385:239-50

135. Shimabukuro TT, Kim SY, Myers TR, Moro PL, Oduyebo T, Panagiotakopoulos L. et al. Preliminary Findings of mRNA Covid-19 Vaccine Safety in Pregnant Persons. N Engl J Med. 2021;384:2273-82

136. Kharbanda EO, Vazquez-Benitez G. COVID-19 mRNA Vaccines During Pregnancy: New Evidence to Help Address Vaccine Hesitancy. JAMA. 2022;327:1451-3

137. Jackson LA, Anderson EJ, Rouphael NG, Roberts PC, Makhene M, Coler RN. et al. An mRNA Vaccine against SARS-CoV-2 — Preliminary Report. N Engl J Med. 2020;383:1920-31

138. Anderson EJ, Rouphael NG, Widge AT, Jackson LA, Roberts PC, Makhene M. et al. Safety and Immunogenicity of SARS-CoV-2 mRNA-1273 Vaccine in Older Adults. N Engl J Med. 2020;383:2427-38

139. Baden LR, El Sahly HM, Essink B, Kotloff K, Frey S, Novak R. et al. Efficacy and Safety of the mRNA-1273 SARS-CoV-2 Vaccine. N Engl J Med. 2020;384:403-16

140. Doria-Rose N, Suthar MS, Makowski M, O'Connell S, McDermott AB, Flach B. et al. Antibody Persistence through 6 Months after the Second Dose of mRNA-1273 Vaccine for Covid-19. N Engl J Med. 2021;384:2259-61

141. Regev-Yochay G, Gonen T, Gilboa M, Mandelboim M, Indenbaum V, Amit S. et al. Efficacy of a Fourth Dose of Covid-19 mRNA Vaccine against Omicron. N Engl J Med. 2022;386:1377-80

142. Kremsner P, Mann P, Bosch J, Fendel R, Gabor JJ, Kreidenweiss A. et al. Phase 1 Assessment of the Safety and Immunogenicity of an mRNA- Lipid Nanoparticle Vaccine Candidate Against SARS-CoV-2 in Human Volunteers. medRxiv. 2020. 2020 11.09.20228551

143. Cromer D, Reynaldi A, Steain M, Triccas JA, Davenport MP, Khoury DS. Relating in vitro neutralisation level and protection in the CVnCoV (CUREVAC) trial. medRxiv. 2021. 2021 06.29.21259504

144. Kremsner PG, Ahuad Guerrero RA, Arana-Arri E, Aroca Martinez GJ, Bonten M, Chandler R. et al. Efficacy and safety of the CVnCoV SARS-CoV-2 mRNA vaccine candidate in ten countries in Europe and Latin America (HERALD): a randomised, observer-blinded, placebo-controlled, phase 2b/3 trial. Lancet Infect Dis. 2022;22:329-40

145. Lane S, Yeomans A, Shakir S. Reports of myocarditis and pericarditis following mRNA COVID-19 vaccination: a systematic review of spontaneously reported data from the UK, Europe and the USA and of the scientific literature. BMJ Open. 2022;12:e059223

146. Larson KF, Ammirati E, Adler ED, Cooper LT, Hong KN, Saponara G. et al. Myocarditis After BNT162b2 and mRNA-1273 Vaccination. Circulation. 2021;144:506-8

147. Shay DK, Shimabukuro TT, DeStefano F. Myocarditis Occurring After Immunization With mRNA-Based COVID-19 Vaccines. JAMA Cardiol. 2021;6:1115-7

148. Bozkurt B, Kamat I, Hotez PJ. Myocarditis With COVID-19 mRNA Vaccines. Circulation. 2021;144:471-84

149. Vidula MK, Ambrose M, Glassberg H, Chokshi N, Chen T, Ferrari VA. et al. Myocarditis and Other Cardiovascular Complications of the mRNA-Based COVID-19 Vaccines. Cureus. 2021;13:e15576

150. Karlsson AC, Humbert M, Buggert M. The known unknowns of T cell immunity to COVID-19. Sci Immunol. 2020 5

151. Gupta RK. Will SARS-CoV-2 variants of concern affect the promise of vaccines?. Nat Rev Immunol. 2021;21:340-1

152. Trombetta CM, Marchi S, Viviani S, Manenti A, Benincasa L, Ruello A. et al. Serum Neutralizing Activity against B.1.1.7, B.1.351, and P.1 SARS-CoV-2 Variants of Concern in Hospitalized COVID-19 Patients. Viruses. 2021;13:1347

153. Fan Y, Li X, Zhang L, Wan S, Zhang L, Zhou F. SARS-CoV-2 Omicron variant: recent progress and future perspectives. Signal Transduct Target Ther. 2022;7:141

154. Cao L, Lou J, Chan SY, Zheng H, Liu C, Zhao S. et al. Rapid evaluation of COVID-19 vaccine effectiveness against symptomatic infection with SARS-CoV-2 variants by analysis of genetic distance. Nat Med. 2022

155. Lopez Bernal J, Andrews N, Gower C, Gallagher E, Simmons R, Thelwall S. et al. Effectiveness of Covid-19 Vaccines against the B.1.617.2 (Delta) Variant. N Engl J Med. 2021;385:585-94

156. Andrews N, Stowe J, Kirsebom F, Toffa S, Rickeard T, Gallagher E. et al. Covid-19 Vaccine Effectiveness against the Omicron (B.1.1.529) Variant. N Engl J Med. 2022;386:1532-46

157. Tregoning JS, Flight KE, Higham SL, Wang Z, Pierce BF. Progress of the COVID-19 vaccine effort: viruses, vaccines and variants versus efficacy, effectiveness and escape. Nat Rev Immunol. 2021;21:626-36

158. McNamara MA, Nair SK, Holl EK. RNA-Based Vaccines in Cancer Immunotherapy. J Immunol Res. 2015;2015:794528

159. Van Nuffel AM, Benteyn D, Wilgenhof S, Pierret L, Corthals J, Heirman C. et al. Dendritic cells loaded with mRNA encoding full-length tumor antigens prime CD4+ and CD8+ T cells in melanoma patients. Mol Ther. 2012;20:1063-74

160. Liu J, Miao L, Sui J, Hao Y, Huang G. Nanoparticle cancer vaccines: Design considerations and recent advances. Asian J Pharm Sci. 2020;15:576-90

161. Laczkó D, Hogan MJ, Toulmin SA, Hicks P, Lederer K, Gaudette BT. et al. A Single Immunization with Nucleoside-Modified mRNA Vaccines Elicits Strong Cellular and Humoral Immune Responses against SARS-CoV-2 in Mice. Immunity. 2020;53:724-32.e7

162. Copur M. Messenger RNA Vaccines: Beckoning of a New Era in Cancer Immunotherapy. Oncology (Williston Park). 2021;35:190-8

163. Hewitt SL, Bai A, Bailey D, Ichikawa K, Zielinski J, Karp R. et al. Durable anticancer immunity from intratumoral administration of IL-23, IL-36γ, and OX40L mRNAs. Sci Transl Med. 2019 11

164. Zhao X, Pan X, Wang Y, Zhang Y. Targeting neoantigens for cancer immunotherapy. Biomark Res. 2021;9:61

165. Wilson KD, Raney SG, Sekirov L, Chikh G, deJong SD, Cullis PR. et al. Effects of intravenous and subcutaneous administration on the pharmacokinetics, biodistribution, cellular uptake and immunostimulatory activity of CpG ODN encapsulated in liposomal nanoparticles. Int Immunopharmacol. 2007;7:1064-75

166. Midoux P, Pichon C. Lipid-based mRNA vaccine delivery systems. Expert Rev Vaccines. 2015;14:221-34

167. Chono S, Li SD, Conwell CC, Huang L. An efficient and low immunostimulatory nanoparticle formulation for systemic siRNA delivery to the tumor. J Control Release. 2008;131:64-9

168. Scioli Montoto S, Muraca G, Ruiz ME. Solid Lipid Nanoparticles for Drug Delivery: Pharmacological and Biopharmaceutical Aspects. Front Mol Biosci. 2020;7:587997

169. Liang F, Lindgren G, Lin A, Thompson EA, Ols S, Röhss J. et al. Efficient Targeting and Activation of Antigen-Presenting Cells In Vivo after Modified mRNA Vaccine Administration in Rhesus Macaques. Mol Ther. 2017;25:2635-47

170. Coelho T, Adams D, Silva A, Lozeron P, Hawkins PN, Mant T. et al. Safety and efficacy of RNAi therapy for transthyretin amyloidosis. N Engl J Med. 2013;369:819-29

171. Wang S-J, Fotenos A, Masters SC, Marzella L. Theranostics approach in drug development: is there study efficiency when the prevalence of the molecular target is very high?. Theranostics. 2022;12:3079-83

172. Elia U, Ramishetti S, Rosenfeld R, Dammes N, Bar-Haim E, Naidu GS. et al. Design of SARS-CoV-2 hFc-Conjugated Receptor-Binding Domain mRNA Vaccine Delivered via Lipid Nanoparticles. ACS Nano. 2021;15:9627-37

173. Kauffman KJ, Mir FF, Jhunjhunwala S, Kaczmarek JC, Hurtado JE, Yang JH. et al. Efficacy and immunogenicity of unmodified and pseudouridine-modified mRNA delivered systemically with lipid nanoparticles in vivo. Biomaterials. 2016;109:78-87

174. Kim M, Jeong M, Hur S, Cho Y, Park J, Jung H. et al. Engineered ionizable lipid nanoparticles for targeted delivery of RNA therapeutics into different types of cells in the liver. 2021; 7: eabf4398.

175. Tao W, Davide JP, Cai M, Zhang GJ, South VJ, Matter A. et al. Noninvasive imaging of lipid nanoparticle-mediated systemic delivery of small-interfering RNA to the liver. Mol Ther. 2010;18:1657-66

176. Farbiak L, Cheng Q, Wei T, Álvarez-Benedicto E, Johnson LT, Lee S. et al. All-In-One Dendrimer-Based Lipid Nanoparticles Enable Precise HDR-Mediated Gene Editing In Vivo. Adv Mater. 2021;33:e2006619

177. Abrams MT, Koser ML, Seitzer J, Williams SC, DiPietro MA, Wang W. et al. Evaluation of efficacy, biodistribution, and inflammation for a potent siRNA nanoparticle: effect of dexamethasone co-treatment. Mol Ther. 2010;18:171-80

178. Ndeupen S, Qin Z, Jacobsen S, Bouteau A, Estanbouli H, Igyártó BZ. The mRNA-LNP platform's lipid nanoparticle component used in preclinical vaccine studies is highly inflammatory. iScience. 2021;24:103479

179. Zhang H, Han X, Alameh M-G, Shepherd SJ, Padilla MS, Xue L. et al. Rational design of anti-inflammatory lipid nanoparticles for mRNA delivery. J Biomed Mater Res A. 2022;110:1101-8

180. Khan ZU, Razzaq A, Khan A, Rehman NU, Khan H, Khan T. et al. Physicochemical Characterizations and Pharmacokinetic Evaluation of Pentazocine Solid Lipid Nanoparticles against Inflammatory Pain Model. Pharmaceutics. 2022;14:409

181. MacRitchie N, Frleta-Gilchrist M, Sugiyama A, Lawton T, McInnes IB, Maffia P. Molecular imaging of inflammation - Current and emerging technologies for diagnosis and treatment. Pharmacol Ther. 2020;211:107550

182. Love C, Tomas MB, Tronco GG, Palestro CJ. FDG PET of Infection and Inflammation. RadioGraphics. 2005;25:1357-68

183. Gouilly D, Saint-Aubert L, Ribeiro M-J, Salabert A-S, Tauber C, Péran P. et al. Neuroinflammation PET imaging of the translocator protein (TSPO) in Alzheimer's disease: An update. Eur J Neurosci. 2022;55:1322-43

184. Shi B, Keough E, Matter A, Leander K, Young S, Carlini E. et al. Biodistribution of small interfering RNA at the organ and cellular levels after lipid nanoparticle-mediated delivery. J Histochem Cytochem. 2011;59:727-40

185. H-J I, GJ C. Preclinical PET and SPECT for Radionanomedicine.. In: DS L, editor. Radionanomedicine: SPRINGER; 2019. p. 279-92

186. Lasa-Saracíbar B, El Moukhtari SH, Tsotakos T, Xanthopoulos S, Loudos G, Bouziotis P. et al. In vivo biodistribution of edelfosine-loaded lipid nanoparticles radiolabeled with Technetium-99 m: Comparison of administration routes in mice. Eur J Pharm Biopharm. 2022;175:1-6

187. Man F, Gawne PJ, R TMdR. Nuclear imaging of liposomal drug delivery systems: A critical review of radiolabelling methods and applications in nanomedicine. Adv Drug Deliv Rev. 2019;143:134-60

188. Lee H, Gaddy D, Ventura M, Bernards N, de Souza R, Kirpotin D. et al. Companion Diagnostic (64)Cu-Liposome Positron Emission Tomography Enables Characterization of Drug Delivery to Tumors and Predicts Response to Cancer Nanomedicines. Theranostics. 2018;8:2300-12

189. Wurtmann EJ, Wolin SL. RNA under attack: cellular handling of RNA damage. Crit Rev Biochem Mol Biol. 2009;44:34-49

190. Sousa de Almeida M, Susnik E, Drasler B, Taladriz-Blanco P, Petri-Fink A, Rothen-Rutishauser B. Understanding nanoparticle endocytosis to improve targeting strategies in nanomedicine. Chem Soc Rev. 2021;50:5397-434

191. Iversen T-G, Skotland T, Sandvig K. Endocytosis and intracellular transport of nanoparticles: Present knowledge and need for future studies. Nano Today. 2011;6:176-85

192. Xu H, Ren D. Lysosomal Physiology. Annu Rev Physiol. 2015;77:57-80

193. Smith SA, Selby LI, Johnston APR, Such GK. The Endosomal Escape of Nanoparticles: Toward More Efficient Cellular Delivery. Bioconjug Chem. 2019;30:263-72

194. Funhoff AM, van Nostrum CF, Koning GA, Schuurmans-Nieuwenbroek NM, Crommelin DJ, Hennink WE. Endosomal escape of polymeric gene delivery complexes is not always enhanced by polymers buffering at low pH. Biomacromolecules. 2004;5:32-9

195. Kongkatigumjorn N, Cortez-Jugo C, Czuba E, Wong ASM, Hodgetts RY, Johnston APR. et al. Probing Endosomal Escape Using pHlexi Nanoparticles. Macromol Biosci. 2017;17:1600248

196. Du Rietz H, Hedlund H, Wilhelmson S, Nordenfelt P, Wittrup A. Imaging small molecule-induced endosomal escape of siRNA. Nat Commun. 2020;11:1809

Author contact

Corresponding authors: Dr. Hyung Jun Im, iiihjjjac.kr; Dr. Hyewon Youn, hwyounac.kr

Received 2022-7-19
Accepted 2022-10-6
Published 2022-10-24

Citation styles

©2024 Ivyspring International Publisher. Terms of use