key: cord-1004677-11ejfiwe
authors: Barnard, Karen N.; Wasik, Brian R.; LaClair, Justin R.; Buchholz, David W.; Weichert, Wendy S.; Alford-Lawrence, Brynn K.; Aguilar, Hector C.; Parrish, Colin R.
title: Expression of 9-O- and 7,9-O-Acetyl Modified Sialic Acid in Cells and Their Effects on Influenza Viruses
date: 2019-12-03
journal: mBio
DOI: 10.1128/mbio.02490-19
sha: 2448743a5de075f6a1816e46fe72b69cc791da18
doc_id: 1004677
cord_uid: 11ejfiwe

Sialic acids (Sia) are widely displayed on the surfaces of cells and tissues. Sia come in a variety of chemically modified forms, including those with acetyl modifications at the C-7, C-8, and C-9 positions. Here, we analyzed the distribution and amounts of these acetyl modifications in different human and canine cells. Since Sia or their variant forms are receptors for influenza A, B, C, and D viruses, we examined the effects of these modifications on virus infections. We confirmed that 9-O-acetyl and 7,9-O-acetyl modified Sia are widely but variably expressed across cell lines from both humans and canines. Although they were expressed on the cell surfaces of canine MDCK cell lines, they were located primarily within the Golgi compartment of human HEK-293 and A549 cells. The O-acetyl modified Sia were expressed at low levels of 1 to 2% of total Sia in these cell lines. We knocked out and overexpressed the sialate O-acetyltransferase gene (CasD1) and knocked out the sialate O-acetylesterase gene (SIAE) using CRISPR/Cas9 editing. Knocking out CasD1 removed 7,9-O- and 9-O-acetyl Sia expression, confirming previous reports. However, overexpression of CasD1 and knockout of SIAE gave only modest increases in 9-O-acetyl levels in cells and no change in 7,9-O-acetyl levels, indicating that there are complex regulations of these modifications. These modifications were essential for influenza C and D infection but had no obvious effect on influenza A and B infection.

others, which may be present individually or in many combinations (1) . Since many different enzymes and pathways introduce these modifications, complex mixtures of Sia forms may be present, with significant variation in both the levels and the specific combinations of each modification (1, 2, 5) .

Common chemical additions include O-acetyl modifications to the C-4, -7, -8, and/or -9 positions, resulting in a variety of combinations, including Neu4,5Ac, Neu5,9Ac 2 , and Neu5,7,9Ac 3 Sia. The addition of O-acetyl modifications (O-Ac) to the C-7 and/or C-9 positions is mediated by the sialate O-acetyltransferase enzyme, Cas1 domain containing 1 (CasD1) (Fig. 1B ). CasD1 appears to add acetyl groups to the C-7 position of Sia, from which it may migrate to the C-8 and C-9 position under physiological conditions, allowing the possible addition of another acetyl group to C-7 (6, 7) . A migrase enzyme has been proposed to aid in the transfer of the acetyl group from C-7 to C-9; however, a specific enzyme has yet to be identified (5, 8, 9) . CasD1 is localized in the late Golgi compartment, so acetyl modifications are added during the later stages of protein glycosylation. The regulatory processes that control the number of acetyl groups added or their positions have not been well defined, although clear differences in expression of 7,9-O-Ac and 9-O-Ac have been reported in mouse and human cells and tissues, in chicken embryos, and in the tissues of some other animals (10, 11) . CasD1 uses acetyl coenzyme A and likely has a preference for CMP-Neu5Ac as a substrate so that it is less active on CMP-Neu5Gc (7) .

At least one sialate O-acetylesterase (SIAE) enzyme regulates the display of 7,9-Oand 9-O-Ac in many cells and tissues (Fig. 1B) . The SIAE gene encodes two isoforms that vary in the presence of a proposed C-terminal localization tag in the lysosomal form (Lse) that is absent from the cytosolic form (Cse) (12) . However, the processes that regulate the expression and activity of these two isoforms remain poorly defined. Lse has been found to localize to the Golgi compartment and/or endoplasmic reticulum (ER) and on the surfaces of cells when overexpressed, with the majority being secreted into the supernatant (12) . Antibody staining shows that Cse is found diffusely throughout the cytosol, where it is thought to remove 9-O-and 7-O-acetyl groups to recycle the Sia for reuse in glycosylation (12) . Despite the reports of distinct protein expression in mouse tissues, bioinformatic analysis of RNA expression in human cells and tissues show mRNA corresponding to the Lse form of SIAE and none responding to the Cse form (13) . It is therefore still unclear how these two isoforms are regulated in humans or other animals, whether their expression relates to CasD1, or what controls the levels and locations of 9-O-and 7,9-O-Ac expression.

Sia O-acetylation and deacetylation play important roles in many different biological processes, particularly in development, cancer, and immunology. For example, O-acetyl modifications to Sia may alter the binding of host lectins, including siglecs (3, 5, 14) . Siglecs are regulators of many different cell functions and developmental processes; examples include B-and T cells, where the presence of 9-O-acetyl Sia modulates immune cell activation and differentiation (15) . In B cells, negative regulation of B-cell receptor (BCR) activation by siglec CD22 is mediated by binding to Neu5Ac-terminated glycan chains on the BCR, which can be blocked by O-acetyl modifications (16, 17) . The presence of 9-O-Ac can also reduce the activity of sialidases, including human neuraminidases (18) . Incorrect regulation of 9-O-Ac, 7,9-O-Ac, and SIAE activity has been linked to autoimmune disorders through the development of autoantibodies (17, 19) . 9-O-Ac and 7,9-O-Ac, and their regulation by SIAE also appear to play important roles during early stages of embryonic development, spermatogenesis, and in different forms of cancer, including acute lymphoblastic leukemia, colon cancer, and breast cancer (20) (21) (22) (23) .

Effects of different Sia modifications have also been suggested for the binding of pathogens or on the activities of their sialidases (neuraminidases). However, in general these are still not well documented, with the exception of those that use the modified forms as receptors. Influenza A virus (IAV), IBV, ICV, and IDV use Sia as their primary receptors for host recognition and cell entry, but with different effects of Sia modification. IAV and IBV interact with Sia through two surface glycoproteins, hemagglutinin (HA) and neuraminidase (NA). For both IAV and IBV, HA binds Sia to initiate the endocytic uptake of the virus by the cell, leading to fusion between the viral envelope and the endosomal membrane at low pH (24, 25) . NA is a sialidase which cleaves Sia off glycan chains when it is present in mucus or on the surface of cells, allowing the virus to penetrate to the epithelial cells and also preventing aggregation of newly produced virus after budding (26, 27) . In contrast to IAV and IBV, ICV and IDV have one surface glycoprotein, the hemagglutinin-esterase fusion protein (HEF), which serves similar purposes to both HA and NA. HEF binds specifically to 9-O-acetyl Sia to initiate uptake of the virus into cells, while the esterase domain removes 9-O-acetyl modifications, releasing the virus from mucus and disassembling virus aggregates after budding (28) (29) (30) (31) . While the role of O-acetyl modified Sia for ICV and IDV infections are well documented, how these modifications affect IAV is not well characterized. In addition, although previous preliminary studies have suggested that the presence of 9-O-Ac on cells may be inhibitory for both NA activity and HA binding of IAV (32, 33) , the details are unclear.

Here, we examine and more closely define the expression and distribution of 9-O-acetyl and 7,9-O-acetyl Sia on cells in culture, define the effects of SIAE and CasD1 on display of these Sia modifications, and perform an initial examination of the effects of these modified Sia on infection by IAV, IBV, ICV, and IDV. We used CRISPR-Cas9 for gene engineering of the enzymes that add or remove the 9-O-and 7,9-O-acetyl groups from Sia and combine these with the recently developed viral protein-derived probes that specifically recognize modified Sia. By merging these with high-pressure liquid chromatography (HPLC)-based quantification of the different Sia forms, we provide a more detailed understanding of the expression and localization of these modifications in cells and examine their effects on host-virus interactions as examples.

There is currently only sporadic information about the expression of modified Sia on commonly used cell lines or an understanding of how that compares to the expression in animal tissues. We examined cell lines that are widely used in many experimental systems: A549 human type II alveolar epithelial cells, HEK-293 human kidney derived cells (possibly embryonic adrenal precursor cells [34] ), and MDCK canine kidney epithelial cells. In addition, we tested MDCK type I and type II cells that were previously subcloned by others from the ATCC MDCK line (MDCK-NBL2) and which have been extensively characterized (35) (36) (37) . We used probes derived from porcine torovirus (PToV) and bovine coronavirus (BCoV) hemagglutinin-esterase proteins (HE) that were fused to human IgG1 Fc and which had the esterase active site inactivated (HE-Fc). The PToV HE-Fc probe recognizes 9-O-Ac, while BCoV HE-Fc recognizes primarily 7,9-O-Ac, although with a low affinity for 9-O-Ac (10, 11) . As observed by immunofluorescence microscopy, the different forms were evident at variable levels, with between 10 and 70% of the cells of each type showing staining under standard culture conditions (Fig. 2) . MDCK-NBL2 and MDCK type I cells showed both strong surface and internal staining for 7,9-O-and 9-O-Ac forms, while both were mostly found in intracellular locations in A549 and HEK-293 cells, with an occasional cell showing bright surface staining. MDCK type II cells showed staining only for 9-O-Ac and none for 7,9-O-Ac, indicating that these modifications are regulated independently. In HEK-293 and A549 cells, both 7,9-O-and 9-O-Ac appeared to be localized within the Golgi compartment, as confirmed by costaining with the Golgi marker GM130 (Fig. 3) . Similar localization differences between some cell lines have been seen previously using the ICV HEF as a probe (38) . In our studies, there was inherent variability within populations in terms of both level of staining and localization. For example, in MDCK-NBL2 not all cells were positive for 9-O-Ac, whereas in MDCK type I some cells retained more 9-O-Ac and 7,9-O-Ac internally, while others displayed more of the modified Sia on their surfaces ( Fig. 2A) . This heterogeneity was consistent between different passages of each cell line.

The expression levels of those modified Sia variants were also quantified by HPLC analysis using DMB (1,2-diamino-4,5-methylenedioxybenzene) labeling and fluorescence detection (39) . The cells were treated at 80˚C for 3 h in the presence of 2 M acetic acid, and therefore the data likely represent the total Sia present in the cells. Even though some cell lines showed strong staining by the HE-Fc probes, the levels of 9-O-Ac were 1 to 2% of the total collected Sia from all cells, while the levels of 7,9-O-Ac were below the level of detection in all cell lines ( Fig. 2 and Table 1 ; see also Fig. S1 in the supplemental material). This includes cells from other species, including cat, mouse, horse, and swine. Unique among the cells tested, A549 cells are secretory and express significant levels of mucin (including MUC1 and MUC5B) (40) . Although mucin proteins are not the only secreted protein found in mucus, we chose to focus on them due to their high levels of glycosylation (80% of weight) and proposed importance as a barrier to pathogens (41) (42) (43) . We found that A549 cells were able to secrete MUC5B into conditioned media (see Fig. S2A in the supplemental material), although we found that the amounts secreted were variable between collections. Analysis of conditioned media from A549 cells showed that approximately 2% of Sia was 9-O-Ac on secreted proteins with no 7,9-O-Ac detected, indicating that, at least in these cells, secreted proteins were not enriched for O-acetylated Sia (Fig. S2B) . However, it would be worth examining proteins secreted by primary cells from humans or that are present in different tissues, including mucins, to determine whether the secreted proteins from A549 are representative of respiratory mucus.

The low levels of 9-O-and 7,9-O-Ac detected on HEK-293, A549, and MDCK cells by HPLC could be due to the heterogeneity of the population, since this method measures total Sia for all cells in the population. However, it is likely that even on cells expressing higher levels of 7,9-O-and 9-O-Ac, these modified Sia make up a small proportion of the total Sia present in the cell or glycocalyx. Previous studies have reported that podo-planin (GP40 in canine cells) is a primary carrier of 9-O-Ac on MDCK cells and therefore acts as the main receptor for ICV (44, 45) . However, when we costained MDCK cells with an anti-podoplanin antibody and PToV HE-Fc, we saw little correlation between podoplanin and 9-O-Ac staining (Fig. S3) .

Production of CasD1 knockout and CasD1-overexpressing cells. To better understand the control of expression of 7,9-O-and 9-O-Ac, glycoengineered cell lines were created by manipulating the expression of CasD1 and SIAE genes. To do this, we knocked out CasD1 via CRISPR-Cas9 editing or overexpressed CasD1 via transfection of an expression plasmid. Knockout variants of CasD1 (ΔCasD1) were prepared from MDCK-NBL2, A549, and HEK-293 cells using CRISPR-Cas9 targeting of early exons in the CasD1 gene (Fig. 4A ). ΔCasD1 clones were confirmed by examining for 7,9-O-and 9-O-Ac display and then by PCR and sequencing of the genomic region surrounding the deletion in modified Sia-negative clones (Fig. 4A ). For all cell types, ΔCasD1 variants showed loss of both 7,9-O-and 9-O-Ac display when probed with the different specific HE-Fc probes via flow cytometry and immunofluorescence microscopy ( Fig. 4B to D). , MDCK type I, and MDCK type II cells. Cells were probed with HE-Fcs probes derived from BCoV and PToV, which recognize 9-O-Ac and 7,9-O-Ac, respectively. Cells were permeabilized (perm) using Carbo-Free blocking reagent with 0.001% Tween 20, while nonpermeabilized cells (non-perm) received only Carbo-Free block. All cells were imaged at ϫ60; nuclei were stained with DAPI. Scale bar, 10 m. (B) Representative flow cytometry graphs showing distribution of positive staining for HEK-293, A549, and MDCK-NBL2 cell lines. BCoV and PToV HE-Fcs probes were used and permeabilization (perm) and nonpermeabilization (non-perm) methods were as in immunofluorescence assay staining.

® This agrees with previous findings that loss of CasD1 leads to loss of both 7,9-O-and 9-O-Ac modifications in haploid HAP1 cells (7) . HPLC analysis of total Sia showed a significant decrease in 9-O-Ac expression compared to wild-type (WT) cells; however, very low levels (Ͻ1%) were still detectable, despite a lack of staining with the HE-Fc probes (Fig. 4E ). This could be due to exogenous Sia from the fetal bovine serum in the growth media, as is the case for Neu5Gc, which is also detectable at similarly low levels on cells even though the gene for Neu5Gc synthesis, CMAH, is not functional in humans or canines (Fig. S1 ) (46, 47) .

Due to the heterogeneity and low expression of 7,9-O-and 9-O-Ac in WT cells, we sought to engineer cells with more homogeneous and higher levels of these modifications. We overexpressed the human CasD1 (CasD1-OX) in the ΔCasD1 variants of MDCK-NBL2, A549, and HEK-293 cells, expecting that expression of CasD1 under a strong promoter in the ΔCasD1 background would increase the consistency of the synthesis and display of 9-O-and 7,9-O-acetyl Sia relative to the WT cells. CasD1-OX cells showed significantly higher levels of CasD1 mRNA compared to WT cells, indicating that the CasD1 expression plasmid was being transcribed at high levels ( Fig. 4E) . However, only a modest increase in average 9-O-and 7,9-O-Ac expression across the population in HEK-293 cells was seen by flow cytometry, whereas fluorescence microscopy showed heterogeneity of expression in the population ( Fig. 4B to D). The transfected MDCK and A549 CasD1-OX cells showed recovery of 9-O-and 7,9-O-Ac synthesis when analyzed by flow cytometry and immunofluorescence microscopy, but the levels were not as high as those seen in WT cells ( Fig. 4B to D). HPLC analysis confirmed the expression levels for HEK-293, A549, and MDCK cells (Fig. 4F ). In addition, heterogeneity was still seen in these populations for 9-O-Ac. This suggests that 7,9-Oand 9-O-Ac expression is not directly regulated by the levels of CasD1 gene expression but may be affected by posttranslational regulation of CasD1 activity or removal of the modifications by SIAE or other enzymes. In addition, these modifications are not regulated the same across individual cells, as evidenced by the population heteroge- Effects of Modified Sialic Acids on Influenza Viruses ® neity. SIAE transcripts were consistently expressed in HEK-293 WT, ΔCasD1, and CasD1-OX cell populations by qPCR analysis, although SIAE mRNA levels in CasD1-OX cells were lower than those seen in WT (Fig. 4E ).

To determine the role of SIAE activity in regulating 7,9-O-and 9-O-Ac display, SIAE knockout (ΔSIAE) cells were generated from WT HEK-293 and A549 cells by targeting early exons in the SIAE gene (Fig. 5A ). Complete knockout of SIAE was confirmed both by genotyping to show deletions in both alleles and by loss of mRNA by qPCR ( Fig. 5A and D) . ΔSIAE cells showed a small but significant increase in surface display and a large increase in internal display of 9-O-Ac based on flow cytometry, but they did not appear to show any changes in the surface or internal display of 7,9-O-Ac ( Fig. 5B and C) . HPLC analysis also showed a small increase of 9-O-Ac in HEK-293 cells, but no 7,9-O-Ac was detected in either cell line (Fig. 5E ). When the overexpression CasD1 plasmid was transfected into ΔSIAE cells (ΔSIAEϩCasD1), the cells showed an increase in both surface and internal 9-O-Ac but no increase in surface or internal display of 7,9-O-Ac by either flow cytometry or immunofluorescence microscopy ( Fig. 5B and C) . HPLC confirmed the flow cytometry results by showing a small increase of 9-O-Ac levels in HEK-293 cells, similar to those seen in CasD1-OX (Fig. 5E) . A549 cells showed a small but nonsignificant increase in 9-O-Ac levels compared to WT by HPLC analysis. Interestingly, HEK-293 ΔSIAEϩCasD1 cells grew more slowly than either ΔSIAE or WT cells (Fig. 5F ). However, A549 ΔSIAEϩCasD1 showed increased growth rates compared to ΔSIAE or WT cells, while ΔSIAE cells had slightly lower growth rates compared to WT. This suggests that 7,9-O-and 9-O-Ac may affect cell metabolism and growth rates and that these effects may be cell type specific. Overall, these results show that SIAE regulates levels of 9-O-Ac and 7,9-O-Ac but that knocking out SIAE only leads to small increases in these modifications. However, there appear to be mechanisms regulating the surface display (Fig. 6C and D) . The C/Ann Arbor and C/Victoria recovered a low level of infectivity in the MDCK CasD1-OX cells, whereas the D/bovine and D/swine strains had a higher level of infectivity recovered in the CasD1-OX cells compared to ICV but still were much lower than in WT MDCK cells. The inability of the ICV and IDV strains to fully recover infectivity may be due to the low surface levels of 9-O-Ac Sia on MDCK CasD1-OX cells. Although the CasD1-OX cells had detectable surface levels of 9-O-Ac, these levels were lower than in WT MDCK cells and could be below the receptor levels required for efficient infection by these viruses. This suggests that ICV and IDV are able to utilize the levels of modified Sia on WT MDCK cells as their primary receptors for binding and infection but cannot infect when they are removed or below a certain necessary threshold.

Effects of 7,9-O-or 9-O-acetyl Sia modifications on HA binding and NA activity. Since the low levels of 7,9-O-and 9-O-AC on the surfaces of cells did not effect IAV infection in our assays, we sought to determine the effects of these modifications on HA binding and NA cleavage using mouse erythrocytes which have ϳ45% of their total Sia is O-acetylated, primarily 7,9-O-and 9-O-Ac (Fig. 7A) . Although mouse erythrocytes contain primarily ␣2,3-linked Sia, they also contain some ␣2,6-linked Sia that could be bound by human IAV strains (Fig. 7A) . Mouse erythrocytes were therefore used as a substrate for both binding (hemagglutination) assays and neuraminidase cleavage assays. The human IAV strains human H1N1 (A/California/04/2009) and human H3N2 (A/Victoria/361/2011) strains were mixed with either untreated mouse erythrocytes or mouse erythrocytes pretreated with esterase active BCV HE-Fc to remove all acetyl modifications (Fig. 7B) . Significantly greater hemagglutination was seen for both viruses on the esterase-treated mouse erythrocytes compared to untreated erythrocytes. It should be noted that the hemagglutination was still quite low, which is likely due to the lower levels of ␣2,6-linked Sia on mouse erythrocytes.

To determine the effect of 7,9-O-and 9-O-Ac on NA cleavage, mouse erythrocytes were incubated with soluble NA, in the form of NA-expressing viruslike particles (VLPs) (48) . Freed Sia was then collected and analyzed using HPLC, and the profile of Sia released by the NA VLPs was compared to Sia composition on mouse erythrocytes released by chemical hydrolysis (Fig. 7C ). The profiles for both N1 and N2 VLPs showed a preferential release of unmodified Neu5Ac compared to modified Sia forms, shown in the increased proportion of this Sia in the N1 and N2 profiles. Compared to the chemical release profile, the N1 VLPs did not release any detectable O-acetylated Sia, while the N2 VLPs were able to release 9-O-Ac (Neu5,9Ac 2 ) but released significantly less 7-O-and 8-O-Ac and were unable to release any 7,9-O-Ac (Neu5,7,9Ac 3 ). Similar to N2 VLPs, commercial NeuA from Arthrobacter ureafaciens, used as an activity control, also had a bias toward unmodified Neu5Ac, with decreased activity against 7-O-, 8-O-, and 7,9-O-Ac. These results indicate that mono O-acetyl modifications, including 7-O-, 8-O-, and 9-O-Ac, reduced the Sia susceptibility to NA cleavage and that diacetyl 7,9-O-Ac was the most resistant to NA cleavage. In addition, there was variability between the ability of the NA VLPs and NeuA to cleave the different Sia forms. Although the presence of these modified Sia on cells was too low to affect IAV infection, it is likely that higher levels present on erythrocytes, or potentially in secreted proteins in mucus, would inhibit infection or the release of virus.

Both 9-O-Ac and 7,9-O-Ac Sia are widely expressed within tissues and on mucosal surfaces of many animals, but with significant variation in the amounts present in different cells, tissues, and animals (10, 11). These modified Sia are present in secreted mucus on mucosal surfaces, including gastrointestinal and respiratory tissues, where they can potentially control many interactions with both normal flora and pathogens. However, there is still little known about the details of their display levels, cell association, and the ways in which their synthesis is regulated either in cells or on mucosal surfaces. While there have been suggestions that 9-O-and 7,9-O-Ac might influence IAV and IBV infection by interfering with HA binding or NA activities, direct evidence for their effects is sparse. In contrast, ICV and IDV are known to use 9-O-Ac as their primary receptor for cell binding and infection. Here, we use a number of new tools to define the cell-specific expression of 9-O-and 7,9-O-Ac and provide a preliminary test of their effects on IAV, IBV, ICV, and IDV infection.

We confirmed that 9-O-and 7,9-O-Ac are expressed on cells in culture and that expression varies between cell lines, as has been previously reported (38) . However, when present these modified Sia made up only 1 to 2% of the total Sia when analyzed by HPLC. Cells showed distinct population heterogeneity in 7,9-O-and 9-O-Ac display and localization that was observed over many passages examined. Previous studies using ICV HEF probes found similar staining patterns on some cell lines and also showed that, after sorting into high and low staining populations, both populations returned to previous levels of heterogeneity within a few passages (11, 38) . Here, we saw that the modified Sia are retained in the Golgi compartments of HEK-293 and A549 cells, although an occasional cell displayed these modified Sia on the surface. It is not clear why these modified Sia are localized in the Golgi body, although perhaps the modifications could block the onward trafficking of glycoproteins to the cell surface. In contrast to the human cell lines, MDCK cells showed many cells expressing 7,9-O-Ac and 9-O-Ac on the cell surface, raising the possibility that trafficking could be cell type or species specific. A summary of the synthesis and localization of 7,9-O-and 9-O-Ac is shown in Fig. 8 .

To look more closely at the expression and roles of 7,9-O-and 9-O-Ac modifications and their effects on viral infections, we prepared glycoengineered cell lines that lacked these modifications or that expressed higher levels of CasD1. A deletion and frameshift in CasD1 completely removed both 9-O-and 7,9-O-Ac expression, confirming this enzyme was responsible for creating both modifications, likely through addition to the C-7 position, from which it migrates to the C-9 position (5, 8, 9) . Adding CasD1 back into the cells by plasmid transfection restored modified Sia expression, but none of the cell clones isolated showed universally higher levels of modified Sia synthesis and population heterogeneity was still seen. The CasD1-transfected HEK-293 cells showed the greatest increase, whereas for A549 and MDCK cells the expression was similar to or lower than that for WT cells. However, even in the HEK-293 CasD1-OX cells, 9-O-Ac still only accounted for ϳ1.5% of total Sia, and 7,9-O-Ac was not detected. This indicates that the levels of these modifications are not only controlled by the expression of CasD1 and could be regulated by other processes. In addition, there is clearly a differential regulation of 7,9-O-Ac compared to 9-O-Ac, as overexpressing CasD1 did not lead to an increase in 7,9-O-Ac, since it was not detectable by HPLC and there was only very low fluorescence via staining with BCoV HE-Fc.

One candidate for control of these modifications is SIAE. When we knocked SIAE out of HEK-293 and A549 cells, we saw an increase in 9-O-Ac that was still retained in the Golgi compartment, but there was no increase in 7,9-O-Ac. Expressing CasD1 from a plasmid in ΔSIAE HEK-293 and A549 cells resulted in an additional small increase in 9-O-Ac that was still Golgi compartment associated, but with little increase in expression on the cell surface. Similar to the CasD1-OX cells, no increase in 7,9-O-Ac was seen in either ΔSIAE and ΔSIAEϩCasD1 cell lines by HPLC analysis. Both ΔSIAEϩCasD1 lines had altered growth rates compared to WT cells: HEK-293 ΔSIAEϩCasD1 had delayed growth rates, while A549 ΔSIAEϩCasD1 had increased growth rates. This suggests that dysregulation of SIAE and CasD1 by gene manipulation affects cell metabolism and growth in a cell-type-specific manner, possibly through the buildup of glycoproteins in the Golgi or through dysregulation of the sialic acid recycling pathway. These effects on cell growth could have implications for cancer and organismal development, since these variant Sia are involved in both these processes (15-17, 20-23, 49) . Further research is needed to determine how 7,9-O-and 9-O-Ac expression is regulated, how they are transported within the ER and Golgi bodies, and what roles they play in cell growth. Of particular interest will be disentangling the individual regulation of 7,9-O-Ac expression compared to 9-O-Ac, since there do seem to be differences in how they are regulated in cells in the present study versus previously reported expression in animal tissues (10, 11) .

Studies with two strains of IAV and two strains of IBV showed no differences in infection efficiency in WT HEK-293 or MDCK-NBL2 cells compared to their ΔCasD1 or CasD1-OX variants. This is not surprising, since Ͼ95% of the Sia is unacetylated Neu5Ac, which can be utilized by IAV and IBV as a receptor for binding and entry. Although the low levels present on cells were not enough to affect either IAV and IBV infection, we did determine that higher levels, such as those found on mouse erythrocytes (ϳ45% O-Ac), were able to block IAV HA binding and decrease IAV NA cleavage efficiency in a strain-dependent manner. It is possible, therefore, that if higher levels are present on secreted proteins in mucus, they could inhibit infection prior to the virus reaching the cell surface. Further analysis of mucus O-acetylation in IAV hosts would be necessary to determine whether 7,9-O-and 9-O-Ac could contribute to the barrier function of mucus in respiratory tissues (41) .

The 1 to 2% of 9-O-Ac on the surfaces of WT MDCK-NBL2 cells was sufficient for ICV and IDV binding and entry, and thus cell susceptibility was lost when CasD1 was inactivated. Interestingly, there does still seem to be a necessary minimum threshold of 9-O-Ac presence needed for some ICV and IDV strains to infect cells, since the C/Ann Arbor and C/Victoria strains were able to infect some MDCK-CasD1 OX cells at a lower level than WT MDCK cells, whereas the C/Taylor strain was not. Similarly, IDV also Effects of Modified Sialic Acids on Influenza Viruses ® showed lower levels of infectivity in MDCK-CasD1 OX cells compared to WT MDCK cells. It is likely that similar results would be seen for other viruses that use these modified Sia as a receptor, including human coronaviruses OC43 and HKU1 (50) .

In summary, we have shown that these modifications are present in different cell lines sourced from different species of animals, but they make up a small minority of the total Sia present. In addition, these modifications vary considerably in their localization and have an inherent heterogeneity within cell populations. While the presence of both 7,9-O-and 9-O-Ac were dependent on the activity of CasD1, the relative proportions, levels of expression, and localization appear to be controlled by more complex mechanisms than simply the expression of CasD1 and SIAE. How this regulated expression affects cell homeostasis is unknown, but it is likely relevant during development, immune responses, and in cancers that show dysregulation of 7,9-O-and 9-O-Ac expression. For viruses such as ICV and IDV that rely on 9-O-Ac for infection, the low levels seen on cell surfaces are sufficient for infection. We found that 7,9-O-and 9-O-Ac do have inhibitory activity on HA binding and NA cleavage when present at higher levels. Although these modifications are present on cell surfaces at levels too low to affect IAV and IBV infection, they are expressed at much higher levels in mucosal tissues and in secreted mucus proteins of many animals, which may provide a more effective barrier (10, 11, (51) (52) (53) . We are currently examining these processes for secreted mucus and other sources in different animals.

Cells and viruses. HEK-293, A549, MDCK-NBL2, MDCK type I, and MDCK type II cells were grown in Dulbecco modified Eagle medium (DMEM) with 5% fetal bovine serum and 50 g/ml gentamicin. HEK-293, A549, and MDCK-NBL2 cells were obtained from the American Type Culture Collection (ATCC). MDCK type I and type II cells were gifts from William Young (University of Kentucky) (35, 37, 54, 55) . Immunofluorescence microscopy and flow cytometry. Cells were stained using probes derived from viral hemagglutinin-esterase proteins fused to human IgG1 Fc (HE-Fc). The porcine torovirus strain 4 HE-Fc (PToV HE-Fc) primarily recognizes 9-O-Ac, and the bovine coronavirus Mebus strain HE-Fc (BCoV HE-Fc) recognizes 7,9-O-Ac and shows low levels of binding to 9-O-Ac (10, 11) . For immunofluorescence microscopy, the cells were seeded onto glass coverslips and incubated overnight at 37°C and 5% CO 2 . Coverslips were fixed in 4% paraformaldehyde (PFA) for 15 min. Coverslips were incubated with Carbo-Free blocking solution (Vector Laboratories) for 1 h at room temperature, with optional permeabilization with 0.001% Tween 20. For staining, HE-Fc probes were precomplexed with Alexa 488-labeled antihuman IgG antibody for 1 h at 4°C and then diluted in Carbo-Free blocking solution to a final concentration of 5 g/ml HE-Fc and a 1:500 dilution of secondary antibody. Cells were stained with HE-Fc/anti-IgG complex for 1 h at room temperature. Coverslips were mounted using Prolong Antifade-Gold with DAPI (4=,6=-diamidino-2-phenylindole; Invitrogen). Cell were imaged using a Nikon TE300 fluorescence microscope. For flow cytometry, cells were seeded onto nonadherent cell culture dishes and incubated overnight at 37°C and 5% CO 2 . Cells were collected using ice-cold phosphate-buffered saline (PBS; HEK-293 and A549 cells) or Accutase (Sigma, MDCK cells) to retain surface glycans and then fixed in 4% PFA for 15 min. The cells were blocked as described above. HE-Fc probes were prepared as described above with final concentrations of 5 g/ml HE-Fc probe and 1:1,200 of anti-IgG. A Guava EasyCyte Plus flow cytometer (EMD Millipore, Billerica, MA) was used to collect data, followed by analysis using FlowJo software (TreeStar, Ashland, OR). Statistical analyses were performed using GraphPad Prism software (v8).

Cell line mutations and characterization. Two methods for utilizing CRISPR-Cas9 were used. For A549 and MDCK cells, paired Cas9 plasmids (PX459; Addgene plasmid 62988) targeted adjacent sites in early exons of CasD1, as diagrammed in Fig. 4A . Plasmids were transfected using TransIT-X2 (Mirus Bio LLC) (8) . For HEK-293 cells, nickase Cas9 plasmids (PX462; Addgene plasmid 62987) were used instead. Transfected cells were selected with puromycin, and single cell clones were screened with PToV-P4 HE-Fc to identify nonstaining variants. Edited sequences were confirmed by PCR amplification of the targeted regions and sequencing the PCR product for each allele. Knockout cell lines were used to prepare overexpression cell lines by transfection of a pcDNA3.1(-) plasmid expressing the complete human CasD1 cDNA open reading frame synthesized by Bio Basic (Markham, Ontario, Canada). Transfected cells were selected with G418, and single-cell clones were screened by staining with PToV-P4 HE-Fc to identify 9-O-Ac positive cell lines. Editing of the SIAE gene followed a protocol for CRISPR-Cas9 similar to that described above, and the gene regions targeted are shown in Fig. 5A . After transfection and selection, cells were cloned, and single-cell clones were screened by direct PCR amplification of the target gene region and analysis of the PCR product size for the edited form of both alleles. Full sequencing of each allele and qPCR were performed to confirm deletion of the gene.

Quantification of Sia variants. The Sia composition of cells were determined by incubating with 2 M acetic acid at 80°C for 3 h, filtration through a Microcon 10-kDa centrifugal filter (Millipore), and drying in a SpeedVac vacuum concentrator. Released Sia were derivatized with DMB (Sigma-Aldrich) for 2.5 h at 50°C (39) . HPLC analysis was performed using a Dionex UltiMate 3000 system with an Acclaim C 18 column (Thermo Fisher) under isocratic elution in 7% methanol, 7% acetonitrile, and 86% water. Sia standards included bovine submaxillary mucin and commercial standards for Neu5Ac and Neu5Gc (Sigma-Aldrich). Statistical analyses were performed in GraphPad Prism software (v8).

Characterization of A549 conditioned media. Conditioned medium from A549 cells was prepared by washing a fully confluent flask of cells to remove any serum and allowing the cells to grow in serum-free medium for 5 to 7 days. The conditioned medium was collected, dialyzed with 3 volumes of PBS, and concentrated using a 30-kDa centrifugal filter (Pall Corporation). The protein concentration was determined by using a Qubit 4 fluorometer (Invitrogen). To determine Muc5B presence, 2-fold dilutions of conditioned media were compared to purified human Muc5B using a 8% SDS-PAGE gel and probed with an anti-human Muc5B antibody (both purified protein and antibody were gifts from Stefan Ruhl, University of Buffalo). Conditioned medium was analyzed for total Sia using the HPLC methods listed above.

qPCR of SIAE and CasD1 expression. RNA from cells was extracted by using EZNA total RNA kit I (Omega Bio-Tek), and cDNA was synthesized using the SuperScript II reverse transcriptase (Invitrogen) standard protocol with oligo(dT) 12-18 primers (Invitrogen). CasD1-and SIAE-specific primers were designed using Geneious (Biomatters, Ltd.). For CasD1, adequate primers could not be targeted around the CRISPR-Cas9 edit site due to the high G/C content. qPCR was performed on a Applied Biosystems StepOnePlus real-time PCR system using Fast SYBR green (Bio-Rad). Data were analyzed using StepOne software (Applied Biosystems, v2.1) and GraphPad Prism statistical analysis software.

Virus infection assays. For infection in HEK-293 cells with IAV, the cells were seeded on coverslips and inoculated with a multiplicity of infection (MOI) of 0.1. Coverslips of inoculated cells were fixed at 24 h, stained for virus using an anti-NP antibody, and costained with DAPI. The percentages of infected cells were determined by imaging coverslips and counting the infected cells per field. Statistical analyses were performed in GraphPad Prism software. For infection in MDCK cells with the influenza A, B, C, and D viruses, cells were seeded into 96-well plates and inoculated for 48 h. The cells were then fixed and stained with a mouse anti-influenza A NP antibody, a mouse anti-influenza B NP antibody (Abcam), a polyclonal mouse anti-influenza C antibody (a gift from Peter Palese, Icahn School of Medicine at Mount Sinai), or a polyclonal rabbit anti-influenza D antibody (a gift from Feng Li, South Dakota State University). The cells were imaged using a Nikon TE300 fluorescence microscope. Images were analyzed for relative infected cell counts using ImageJ (NIH and LOCI, University of Wisconsin).

Mouse erythrocyte hemagglutination and lectin staining. Mouse erythrocytes were collected from C57B/6 mice by euthanizing the mice and immediately collecting blood by heart puncture into Alsever's solution. Erythrocytes were washed in PBS three times and diluted to 5% (vol/vol) in PBS. Then, 5% of the mouse erythrocytes were left untreated or treated with 30 g/ml BCoV HE-Fc for 18 h at 37°C, followed by dilution to 0.75% (vol/vol) in PBS for the HA assays. Briefly, HA assays were performed by 2-fold serially diluting virus in duplicate per treatment in a V-bottom 96-well plate. Treated or untreated mouse erythrocytes were added to virus and allowed to hemagglutinate at 4°C to prevent NA cleavage. To determine Sia linkage type, 5% washed erythrocytes were blocked for 1 h using 1ϫ Carbo Free blocking buffer (Vector Laboratories) and then stained for 1 h with fluoroscein-labeled plant lectins SNA, which binds ␣2,6-linked Sia, and MAA I, which binds ␣2,3-linked Sia (Vector Laboratories). Stained erythrocytes were then analyzed using flow cytometry as described above.

Generation of NA VLPs and NA cleavage assay. NA sequences were obtained from GenBank (N1, ACP44181; N2, AGC70842). Sequences were tagged, codon optimized, and ordered through Biomatik in the PcDNA3.1(ϩ) vector. To produce VLPs, HEK-293T cells were seeded in 15-cm plates and transfected when 80% confluent. The cells were transfected with 4 l of polyethylenimine (Polysciences, catalog no. 23966-2) at 1 mg/ml for every 1 g of plasmid DNA stock of in 9 ml of Opti-MEM. At 8 h posttransfection, 6 ml of prewarmed Opti-MEM was added. The supernatant was collected at 72 h posttransfection and purified using ultracentrifugation (110,000 ϫ g, 1.5 h, 4°C) through a 20% sucrose cushion. The pellet was resuspended in PBS and stored at 4°C. To determine NA cleavage on mouse erythrocytes, 5% (vol/vol) mouse erythrocytes in PBS were treated with 1:100 NA VLPs for 4 h at 37°C. Free Sia were collected and prepared for HPLC analysis as described above.

Supplemental material for this article may be found at https://doi.org/10.1128/mBio .02490-19. 

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We thank Wendy Weichert for expert technical support and Brynn Lawrence for HA-Fc production.

This work was supported in part by the Center of Research in Influenza Pathogenesis, a NIAID-funded Center of Excellence in Influenza Research and Surveillance contract (HHSN272201400008C to Daniel R. Perez and C.R.P.), NIH grant R01 GM080533 to C.R.P., and an NIH Common Fund Grant (U01CA199792) to Ajit Varki.